United States Environmental Protection Agency
Office of Water
Office of Environmental Information
Washington, DC
EPA-841-R-09-003
National Coastal Condition Assessment
Field Operations
Manual
April 23, 2010
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
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NOTICE
The intention of the National Coastal Condition Assessment project is to provide a
comprehensive assessment for coastal waters across the United States. The complete
documentation of overall project management, design, methods, and standards is contained in
four companion documents:
National Coastal Condition Assessment: Quality Assurance Project Plan (EPA-841-R-0-004)
National Coastal Condition Assessment: Site Evaluation Guidelines
National Coastal Condition Assessment: Field Operations Manual (EPA-841-R-09-003)
National Coastal Condition Assessment: Laboratory Methods Manual (EPA-841-R-09-002)
This document (Field Operations Manual) contains a brief introduction and procedures to
follow at the base location and on-site, including methods for sampling water chemistry (grabs
and in situ measurements), benthic macroinvertebrates, sediment composition and toxicity, fish
tissue, a pathogen indicator, and physical habitat. These methods are based on the guidelines
developed and followed in the Coastal 2000 and National Coastal Assessment Monitoring and
Assessment Program (USEPA, 2001), Methods described in this document are to be used
specifically in work relating to the National Coastal Condition Assessment. All Project
Cooperators must follow these guidelines. Mention of trade names or commercial products in
this document does not constitute endorsement or recommendation for use. Details on specific
methods for site evaluation and sample processing can be found in the appropriate companion
document.
The citation for this document is:
USEPA. 2009. NATIONAL COASTAL CONDITION ASSESSMENT: FIELD OPERATIONS
MANUAL. EPA-841-R-09-003. U.S. ENVIRONMENTAL PROTECTION AGENCY,
WASHINGTON, DC.
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TABLE OF CONTENTS
ACRONYMS/ABBREVIATIONS viii
CONTACT LIST ix
1.0 NATIONAL COASTAL CONDITION ASSESSMENT BACKGROUND 1
1.1 Survey Design 1
1.1.1 Target Population and Sample Frame 2
1.1.2 Replacing Sites 3
1.2 Selection of NCCA Indicators 3
1.3 Description of NCCA Indicators 3
1.4 Supplemental Material to the Field Operations Manual 5
2.0 DAILY OPERATIONS SUMMARY 7
2.1 Sampling Scenario 7
2.2 Recording Data and Other Information 12
2.3 Safety and Health 14
2.3.1 General Considerations 14
2.3.2 Safety Equipment 16
2.3.3 Safety Guidelines for Field Operations 16
3.0 BASE SITE ACTIVITIES 18
3.1 Predeparture Activities 19
3.1.1 Daily Itineraries 19
3.1.2 Instrument Checks and Calibration 19
3.1.3 Equipment and Supply Preparation 20
3.1.4 Chill Enterococci Filter Extraction Tubes 21
3.2 Post Sampling Activities 21
3.2.1 Post-measurement Calibration Check of Multi-probe Meter 21
3.2.2 Review Data Forms and Labels 22
3.2.3 Inspect and Prepare Samples 22
3.2.4 Equipment Cleanup and Check 22
3.2.5 Shipment of Samples and Forms 24
3.2.5.1 Samples 24
3.2.5.2 Field Forms 25
3.2.6 Status Reports and Communications 25
3.2.6.1 Sample Status Report 25
3.2.6.2 Tracking Forms 25
3.2.6.3 Methods of Communication 26
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TABLE OF CONTENTS (continued)
4.0 INITIAL SITE PROCEDURES 32
4.1 Site Verification Activities 32
4.1.1 Locating the X-Site 32
4.1.2 Target Population 32
4.1.3 Site Verification 33
4.1.4 Site Relocation 34
4.1.5 Sample Collection 35
4.1.6 Secondary Sediment Collection Areas 35
4.1.7 Habitat Assessment 36
4.1.8 Site Photograph 36
5.0 WATER QUALITY MEASUREMENTS 40
5.1 Water Quality 40
5.1.1 In Situ Measurements of Dissolved Oxygen, pH, Temperature, Salinity,
Conductivity, Transparency, and Light Attenuation 40
5.1.1.1 Summary of Method 40
5.1.1.2 Equipment and Supplies 40
5.1.1.3Secchi Disk 43
5.1.1.4 Multi-Probe Sonde 43
5.1.1.5 Photosynthetically Active Radiation (PAR) Meter 46
5.2 Fecal Indicator (Enteroccoci) 47
5.2.1 Summary of Method 47
5.2.2 Equipment and Supplies 47
5.2.3 Sampling Procedure 48
5.3 Water Chemistry Sample Collection and Preservation 48
5.3.1 Summary of Method 48
5.3.2 Equipment and Supplies 49
5.3.3 Sampling Procedure 49
5.4 Phytoplankton Sample Collection and Preservation 50
5.4.1 Summary of Method 50
5.4.2 Equipment and Supplies 50
5.4.3 Sampling Procedure 50
5.5 Underwater Video 51
5.5.1 Summary of Method 51
5.5.2 Equipment and Supplies 51
5.5.3 Initial Setup of Underwater Camera System 52
5.5.4 Underwater Video Recording Procedures 53
6.0 SEDIMENT COLLECTIONS 56
6.1 Sediment Collections 56
6.1.1 Summary of Method 56
6.1.2 Equipment and Supplies 57
6.1.3 Sampling Procedure 58
6.2 Benthic Macroinvertebrate Composition and Abundance 59
6.2.1 Field Processing of Benthic Macroinvertebrate Samples 59
6.3 Sediment Composition, Chemistry and Toxicity 62
6.3.1 Field Processing of Sediment Samples for Chemistry and Toxicity Testing ....62
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TABLE OF CONTENTS (continued)
7.0 FISH TISSUE COLLECTION 64
7.1 Ecological Contamination Fish Collection 64
7.1.1 Equipment and Supplies for Eco Fish Tissue Sampling 64
7.1.2 Sampling Procedure 65
7.2 Summary of Method for Human Health Fish Tissue Sampling 71
8.0 FINAL SITE ACTIVITIES 76
8.1 General Site Assessment 77
8.1.1 Shoreline Activities and Disturbances 77
8.1.2 Site Characteristics 77
8.1.3 General Assessment 77
8.2 Processing the Fecal Indicator and Chlorophyll-a Samples 79
8.2.1 Equipment and Supplies (Fecal Indicator) 79
8.2.2 Procedures for Processing the Fecal Indicator Sample 79
8.2.3 Equipment and Supplies (Chlorophyll-a and Dissolved Nutrients Sample) 81
8.2.4 Procedures for Processing Chlorophyll-a and Dissolved Nutrients Sample 82
8.3 Data Forms and Sample Inspection 83
8.4 Launch Site Cleanup 83
9.0 FIELD QUALITY CONTROL 84
9.1 Repeat Sampling 84
9.2 Field Evaluation and Assistance Visits 84
9.2.1 Specifications for QC Assurance 85
9.2.2 Reporting 86
10.0 LITERATURE CITED 87
APPENDIX A-LIST OF EQUIPMENT AND SUPPLIES A-1
APPENDIX B-FIELD FORMS B-1
APPENDIX C - EXAMPLE OF GREAT LAKES DISINFECTION PROTOCOLS C-1
APPENDIX D-SHIPPING AND TRACKING GUIDELINES D-1
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LIST OF TABLES
Table 2-1 Guidelines for Recording Field Measurements and Tracking Information 13
Table 2-2 General Health and Safety Considerations 15
Table 2-3 General Safety Guidelines for Field Operations 17
Table 3-1 Initial Setup Procedures for LI-COR LI-1400 Datalogger 20
Table 3-2 Stock Solutions, Uses, and Methods for Preparation 21
Table 3-3 Postsampling Equipment Care 23
Table 4-1 Equipment and Supplies List for Site Verification 32
Table 4-2 Site Verification Procedures 39
Table 5-1 Equipment and SuppliesDO, pH, Temperature, Salinity/Conductivity,
Transparency, and Light Attenuation 40
Table 5-2 Sampling ProcedureSecchi Disk 43
Table 5-3 Sampling ProcedureTemperature, pH, Dissolved Oxygen and
Salinity/Conductivity 45
Table 5-4 Sampling ProcedureLight Attenuation 46
Table 5-5 Equipment and Supplies List for Fecal Indicator Sampling 47
Table 5-6 Procedure for Fecal Indicator (Enterococci) Sample Collection 48
Table 5-7 Equipment and Supplies-Water Chemistry and Chlorophyll Sample Collection.. 49
Table 5-8 Sampling Procedure for Water Chemistry and Chlorophyll Sample Collection ..49
Table 5-9 Equipment and SuppliesPhytoplankton 50
Table 5-10 Sampling and Preservation Procedure for Phytoplankton 50
Table 5-11 Equipment and SuppliesUnderwater Video 51
Table 5-12 Initial Setup of Camera System GPS 52
Table 5-13 Procedure for Recording Underwater Video 53
Table 5-14 Procedure for Archiving Underwater Video Files 54
Table 6-1 Equipment and SuppliesSediment Collection 57
Table 6-2 Sampling Procedure for Sediment Collection 58
Table 6-3 Processing Procedure for Benthic Macroinvertebrate Samples 60
Table 6-4 Processing Procedure for Sediment Composition, Chemistry and
Toxicity Testing 63
Table 7-1 Equipment and SuppliesEco Fish Tissue Collection 65
Table 7-2 Recommended Great Lakes Target Species for Whole Body Fish Tissue
Collection by Lake 66
Table 7-3 Recommended Marine Target Species for Whole Body Fish Tissue
Collection by Specific Biogeographical Region 67
Table 7-4 Sampling Procedure for Eco Fish Tissue Composite Samples 67
Table 7-5 Equipment and SuppliesHuman Health Fish Tissue Collection 71
Table 7-6 Target Fish Species for Great Lakes Human Health Fish Tissue Composites ... 72
Table 7-7 Sampling Procedures for Human Health Fish Tissue Composite Samples 73
Table 8-1 Equipment and Supplies List for Fecal Indicator Sample 79
Table 8-2 Processing ProcedureFecal Indicator Sample 80
Table 8-3 Processing ProcedureFilter Blanks 81
Table 8-4 Equipment and Supplies List for Chlorophyll-a and Dissolved
Nutrients Processing 81
Table 8-5 Processing ProcedureChlorophyll-a and Dissolved Nutrients Sample 82
Table 9-1 General Information Noted during Field Evaluation 85
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LIST OF FIGURES
Figure 2-1 Field Sampling Scenario for Teams Using Active Fishing Methods 9
Figure 2-2 Field Sampling Scenario for Teams Using Passive Fishing Methods 10
Figure 2-3 Field Sampling Scenario for Teams not Collecting Fish for Tissue Chemistry.... 11
Figure 2-4 Example Sample Labels for Sample Tracking and Identification 12
Figure 3-1 Overview of Base Site Activities 18
Figure 3-2 Example Tracking and Sample Status Form 28
Figure 3-3 Example Batched Sample Tracking Form 29
Figure 3-4 Example Ecological Fish Tissue Tracking Form 30
Figure 3-5 Example Human Health Fish Tissue Tracking Form 31
Figure 4-1 Example of an Estuarine System 33
Figure 4-2 Example of an Inter-coastal Estuarine System 33
Figure 4-3 Example Site Verification Form (Front) 37
Figure 4-4 Example Site Verification Form (Back) 38
Figure 5-1 Example Field Measurement Form (Front) 41
Figure 5-2 Example Field Measurement Form (Back) 42
Figure 5-3 Setup Diagram of Underwater Video System 52
Figure 5-4 Example Sample Collection Form (Front) 55
Figure 6-1 Illustration of Acceptable and Unacceptable Grabs for Benthic Community
Analysis 59
Figure 6-2 Example Sample Collection Form (Back) 61
Figure 7-1 Example Eco Fish Collection Form (Front) 69
Figure 7-2 Example Eco Fish Collection Form (Back) 70
Figure 7-3 Example Human Health Fish Collection Form (Front) 74
Figure 7-4 Example Human Health Fish Collection Form (Back) 75
Figure 8-1 Final Site Activities Summary 76
Figure 8-2 Example Site Assessment Form 78
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ACRONYMS/ABBREVIATIONS
CPR cardiopulmonary resuscitation
Dl deionized
DO dissolved oxygen
DVR digital video recorder
EMAP Environmental Monitoring and Assessment Program
EPA Environmental Protection Agency
GED Gulf Ecology Division, U.S. EPA Office of Research and Development
GIS geographic information system
GL Great Lakes
GPS global positioning system
GRTS Generalized Random Tessellation Stratified survey design
HOPE high density polyethylene
MED Mid-Continent Ecology Division, U.S. EPA Office of Research and Development
NAD North American Datum
NAWQA National Water-Quality Assessment Program
NCA National Coastal Assessment
NCCA National Coastal Condition Assessment
NEP National Estuaries Program
NHD National Hydrography Dataset
NIST National Institute of Standards
NM Nautical miles
NOAA National Oceanographic and Atmospheric Administration
NRSA National Rivers and Streams Assessment
ORD Office of Research and Development, U.S. EPA
OSHA Occupational Safety and Health Administration
PAH Polycyclic aromatic hydrocarbon
PAR Photosynthetically active radiation
PFD personal floatation device
PSI pounds per square inch
QAPP Quality Assurance Project Plan
QA/QC quality assurance/quality control
QCS Quality Check Solution
SAV Submerged aquatic vegetation
SOPs Standard Operating Procedures
TOC total organic carbon
TP total phosphorus
TSS total suspended solids
USGS United States Geological Survey
WSA Wadeable Streams Assessment
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Jennifer Under
Tetra Tech
400 Red Brook Blvd., Suite 200
Owings Mills, MD, 21117
410-356-8993
410-356-9005 (fax)
Jennifer.Linder@tetratech.com
Sampling Kit Request and Coordination
Mailee Garton
Or
Sara McNew
Great Lakes Environmental Center
739 Hastings St
Traverse City, Ml 49686
231-941-2230
231-941-2240 (fax)
mgarton@glec.com
CONTACT LIST
Field Logistics Coordinators
Chris Turner
Great Lakes Environmental Center
739 Hastings St
Traverse City, Ml 49686
715-829-3737
715-874-5389 (fax)
cturner@glec.com
Information Management Coordinator
Marlys Cappaert
SRA
200 S.W. 35th Street
Corvallis, OR 97333
541-754-4467
541-754-4799 (fax)
cappaert.marlys@epa.gov
Great Lakes Human Health Fish Tissue Contacts
Leanne Stahl
U.S. EPA Office of Water
1200 Pennsylvania Avenue, NW(4503T)
Washington, D.C. 20460
202-566-0404
stahl.leanne@epa.gov
Elaine Snyder
Tetra Tech
400 Red Brook Blvd., Suite 200
Owings Mills, MD, 21117
410-356-8993
blaine.snyder@tetratech.com
Great Lakes Human Health Fish Tissue Sampling Kit Request and Coordination
Tara Kolodiej Carolina Gallardo
Tetra Tech Tetra Tech
400 Red Brook Blvd., Suite 200 400 Red Brook Blvd., Suite 200
Owings Mills, MD, 21117 Owings Mills, MD, 21117
410-356-8993 410-356-8993
tara.kolodiej@tetratech.com carolina.gallardo@tetratech.com
USEPA HEADQUARTERS
Greg Colianni
USEPA Office of Water
Office of Wetlands, Oceans and Watersheds
1200 Pennsylvania Avenue, NW(4503T)
Washington, D.C. 20460
202-566-1249
colianni.gregory@epa.gov
Treda Grayson
USEPA Office of Water
Office of Wetlands, Oceans and Watersheds
1200 Pennsylvania Avenue, NW(4503T)
Washington DC 20460
202-566-0916
grayson.treda@epa.gov
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USEPA REGIONAL CONTACTS
USEPA Region 1
Hilary Snook
617-918-8670
snook.hilary@epa.gov
Diane Switzer
617-918-8377
switzer.diane@epa.gov
USEPA Region 1 - New England Regional
Laboratory
11 Technology Drive
North Chelmsford, MA 01863-2431
USEPA Region 3
Larry Merrill
USEPA Region 3
1650 Arch Street
Philadelphia, PA 19103-2029
215-814-5452
merrill.larry@epa.gov
USEPA Region 2
Darvene Adams
USEPA Facilities
Raritan Depot
2890 Woodbridge Avenue
Edison, NJ 08837-3679
732-321-6700
adams.darvene@epa.gov
USEPA Region 4
David Melgaard
USEPA Region 4
61 Forsyth Street, S.W.
Atlanta, GA 30303-8960
404-562-9265
melgaard.david@epa.gov
USEPA Region 5
Mari Nord
USEPA Region 5
77 West Jackson Boulevard
Chicago, IL 60604-3507
312-886-3017
nord.mari@epa.gov
USEPA Region 9
Janet Hashimoto
USEPA Region 9
75 Hawthorne Street
San Francisco, CA 94105
415-972-3452
hashimoto.janet@epa.gov
USEPA Region 6
Mark Stead
214-665-2271
stead .mark@epa.gov
Laura Hunt
214-665-9729
hunt.laura@epa.gov
USEPA Region 6
1445 Ross Avenue
Suite 1200
Dallas, TX 75202-2733
USEPA Region 10
Gretchen Hayslip
USEPA Region 10
1200 Sixth Avenue
Seattle, WA 98101
206-553-1685
hayslip.gretchen@epa.gov
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1.0NATIONAL COASTAL CONDITION ASSESSMENT BACKGROUND
The National Coastal Condition Assessment (NCCA) is one of a series of water
assessments being conducted by states, tribes, the U.S. Environmental Protection Agency
(EPA), and other partners. In addition to coastal waters, the National Aquatic Resource Surveys
(NARS) also focuses on rivers and streams, lakes, and wetlands in a revolving sequence. The
purpose of these assessments is to generate statistically-valid reports on the condition of our
Nation's water resources and identify key stressors to these systems.
The goal of NARS is to address two key questions about the quality of the Nation's coastal
waters:
What percent of the Nation's coastal waters are in good, fair, and poor condition for key
indicators of water quality, ecological health, and recreation?
What is the relative importance of key stressors such as nutrients and contaminated
sediments?
The NCCA is designed to be completed during the index period of June through the end of
September. Field crews will collect a variety of measurements and samples from predetermined
sampling locations that are determined with an assigned set of coordinates.
This manual describes field protocols and daily operations for crews to use in the NCCA.
The NCCA is a probability-based survey of our Nation's coastal and estuarine waters, and is
designed to:
Assess the condition of the Nation's coastal and estuarine waters at national and
regional scales, including the Great Lakes;
Identify the relative importance of selected stressors to coastal and estuarine water
quality;
Evaluate changes in condition from previous National Coastal Assessment's (NCA)
starting in 2000; and
Help build State and Tribal capacity for monitoring and assessment and promote
collaboration across jurisdictional boundaries.
1.1 Survey Design
EPA selected sampling locations using a probability based survey design. Sample surveys
have been used in a variety of fields (e.g., election polls, monthly labor estimates, forest
inventory analysis) to determine the status of populations or resources of interest using a
representative sample of a relatively few members or sites. Using this survey design allows data
from a subset of sampled sites to be applied to the larger target population, and permits
assessments with known confidence bounds.
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The objectives, or design requirements, for the National Coastal Condition Assessment are
to produce:
estimates of the 2010 status of all coastal waters nationally and regionally (major estuary
groups and the Great Lakes); and
estimates of the change in status in coastal waters between 2010 and 2003, nationally
and regionally (i.e. major estuary groups).
With input from the states and other partners, EPA used an unequal probability design to
select 682 coastal sites and 225 Great Lakes sites. Approximately 10% of the sites are selected
for a return or repeat visit during the index period for quality assurance purposes.
Stratification of NCCA sites is based on major estuaries using the NOAA Coastal
Assessment framework and National Estuary Program (NEP). The Great Lakes sites are
stratified based on the individual Great Lake, depth zone and country. Only the shallow
nearshore depth zone is included in the design for NCCA Great Lakes sites. The shallow
nearshore depth zone is defined as the region extending from the shoreline to a depth of 30 m,
and no more than 5 km from the shoreline.
An "oversample" of additional sites also is available so that any state wishing to conduct a
state level or NEP-level design could be accommodated and to provide alternate sampling sites
if specific sites are rejected. Sites were also identified for the Canadian nearshore although
sampling of these sites is not a part of the NCCA.
1.1.1 Target Population and Sample Frame
The target population for the marine coasts consists of all coastal waters of the
conterminous United States from the head-of-salt to confluence with the ocean, including inland
waterways and major embayments such as Florida Bay and Cape Cod Bay. For the purposes of
this study the head of salt is defined as < .05 parts per thousand (ppt) salinity. The target
population for the Great Lakes consists of all waters of the Great Lakes of the United States and
Canada. The current target population is restricted to the shallow nearshore zones of Lake
Superior, Lake Michigan, Lake Huron, Lake Erie, and Lake Ontario. The NCCA Great Lakes
sites are restricted to the United States portions. Please refer to the Site Evaluation Guidelines
and the NCCA Web site (http://www.epa.gov/owow/monitoring/nationalsurveys.html) for more
detailed information on the target population.
The sample frame was derived from prior National Coastal Assessments developed by EPA
Office of Research and Development (ORD) Gulf Ecology Division (GED). The prior GED
sample frame was enhanced as part of the National Coastal Monitoring Network design by
including information from NOAA's Coastal Assessment Framework, boundaries of National
Estuary Programs and identification of major coastal systems. For NCCA 2010 information on
salinity zones was obtained from NOAA. For Delaware Bay, Chesapeake Bay, Puget Sound
and state of South Carolina, the prior NCA sample frames were replaced by GIS layers provided
by those organizations, ensuring that prior areas sampled in NCA were not excluded and any
differences from the previous sample frames to the current sample frame are clearly identified
in this 2010 NCCA sample frame. The sample frame for the Great Lakes sites were obtained
from EPA ORD Mid-Continent Ecology Division (MED).
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1.1.2 Replacing Sites
It is likely that some sites will be determined to be unsampleable, therefore, a number of
backup sites are provided in the form of an oversample list that is provided to each state. A site
can be deemed unsampleable for any number of reasons, including being too shallow to
properly operate sampling equipment, in the middle of a navigational channel where it is unsafe,
or practically on top of a neighboring site. When a site is determined to be unsampleable,
please document the sampling status of the site and select the next backup station on the list for
that state and estuary type. This maintains the probabilistic integrity of the survey. Please refer
to the Site Evaluation Guidelines for more detailed information on determining site sampling
status.
If a site is generally sampleable, but one or more indicators cannot be collected (e.g. no fish
caught or site is too deep to collect sediment), the site should not be dropped. Rather, the crew
will flag that indicator and document the reason why the indicator could not be collected. See
Section 4.1.6 for information regarding the collection of sediment samples.
1.2 Selection of NCCA Indicators
Indicators for the 2010 survey will basically remain the same as those used in the historic
National Coastal Condition Report with a few modifications. The most prominent change in this
year's survey is the inclusion of coasts along the Great Lakes. Therefore both sample collection
methods and laboratory methods will reflect freshwater and saltwater matrices.
The NCCA workgroup decided on a few changes to the original indicators based on
recommendations from a state and tribal workshop held in 2008 and other discussions. The
changes are: 1) Enterococcus will be collected as a human health indicator; 2) for sediment
toxicity testing, lab methods will use Leptochirus instead ofAmpelisca sp. for saline sites and
Hyalella for freshwater sites; 3) tissue studies will be conducted using whole fish, and 4) the
NCCA will not include the collections of samples for fish community structure, Total Suspended
Solids (TSS), or PAHs in fish tissue.
1.3 Description of NCCA Indicators
In Situ Water Quality Measurements
Measurements for temperature, pH, dissolved oxygen (DO), salinity (at marine sites) and
conductivity (at freshwater sites) will be taken with a calibrated water quality meter or multi-
probe sonde at each site. Measurements will be taken at specific depth intervals at the X-site.
This information will be used to detect extremes in condition that might indicate impairment.
Light Attenuation
A Photosynthetically Active Radiation (PAR) meter, will be used to obtain a vertical profile of
light in order to calculate the light attenuation coefficient at each station. PAR measurements
are taken at the same depths as other water column indicators.
Secchi Disk Transparency
A Secchi disk is a commonly used black and white patterned disk used to measure the
clarity of water within a visible distance.
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Water Chemistry and Associated Measurements
Water chemistry measurements will be used to determine nutrient enrichment, as well as
classification of trophic status. Parameters measured include total and dissolved nitrogen and
phosphorus.
Chlorophyll-a
Chlorophyll-a is the pigment that makes plants and algae green. Its measurement is used to
determine algal biomass in the water.
Dissolved Nutrients
A portion of the filtrate produced from the processing of the chlorophyll-a sample will be
collected in the field and processed in the laboratory for dissolved nutrients.
Phytoplankton Assemblage
Phytoplankton are plant microorganisms that float in the water, such as certain algae,
and are the primary source of energy in most lake systems (Schriver et al. 1995).
Phytoplankton are highly sensitive to changes in ecosystems (e.g., turbidity and nutrient
enrichment). Phytoplankton will be collected in Great Lakes sites only.
Underwater Video
At Great Lakes sites only, crews will use an underwater video camera with recorder to
capture 1 minute of video focused on the substrate at the X-site. Video will be used in the lab to
visually document the bottom composition, and record the presence or absence of zebra
mussels, Cladophora, or other organisms.
Sediment Assessment
Sediment grab samples will be obtained to measure sediment composition (e.g., grain size,
percent moisture, organic content, etc.), toxicity and chemistry in order to determine sediment
condition.
Benthic Macroinvertebrate Assemblage
Benthic macroinvertebrates are bottom-dwelling animals without backbones ("invertebrates")
that are large enough to be seen with the naked eye ("macro"). Examples of macroinvertebrates
include: aquatic worms, mollusks, and crustaceans. Populations in the benthic assemblage
respond to a wide array of stressors in different ways so that it is often possible to determine the
type of stress that has affected a macroinvertebrate assemblage (Klemm et al., 1990). Because
many macroinvertebrates have relatively long life cycles of a year or more and are relatively
immobile, the structure of the macroinvertebrate assemblage is a response to exposure of
present and/or past conditions. The benthic macroinvertebrate data will serve as the basis for
assessing aquatic community health.
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Habitat Assessment
The habitat assessment of the site provides information about the type of habitat located at
a site. This assessment includes presence/absence of submerged aquatic vegetation, marine
debris, and the basic habitat type (e.g., open water, tidal flat, marina, harbor, inlet, tidal
river/stream, seagrass bed, sandy/muddy bottom, rocky bottom, shelly bottom, coral reef, etc.)
Fecal Indicator (Enterococci)
Enterococci are bacteria that are endemic to the guts of warm blooded creatures. These
bacteria, by themselves, are not considered harmful to humans but often occur in the presence
of potential human pathogens (the definition of an indicator organism). Epidemiological studies
of marine and fresh water bathing beaches have established a direct relationship between the
density of Enterococci in water and the occurrence of swimming-associated gastroenteritis.
Fish Tissue
The fish tissue indicator, which measures bioaccumulation of persistent toxics, is used to
estimate the ecological risks associated with fish consumption by wildlife. In this study, fish will
be collected and whole body tissue will be homogenized and analyzed to estimate
concentrations of target contaminants. Various studies have been conducted on contaminants
in different tissues of the fish (e.g., whole fish, fillets, or livers). For this study, the focus will be
on analyzing whole fish for contaminants to generate data for ecological purposes.
In the Great Lakes only, additional fish composite samples will be collected at 150 of the
225 sites (ideally the first 30 sites per lake). Fillet tissue from these samples will be
homogenized and analyzed to generate fish contamination data related to human health.
1.4 Supplemental Material to the Field Operations Manual
The Field Operations Manual describes field protocols and daily operations for crews to use
in the NCCA. Following these detailed protocols will ensure consistency across regions and
reproducibility for future assessments. Before beginning sampling at a site, crews should
prepare a packet for each site containing pertinent information to successfully conduct
sampling. This includes a road map or navigation chart and a set of directions to the site,
topographic/bathymetric maps, land owner access forms (where applicable), sampling permits
(if needed), site evaluation forms and other information necessary to ensure an efficient and
safe sampling day.
Field crews will also receive a quick-reference handbook that contains tables and figures
summarizing field activities and protocols from the Field Operations Manual. This waterproof
handbook will be the primary field reference used by field teams after completing the required
field training session. The field teams are also required to keep the field operations manual
available in the field for reference and for possible protocol clarification, as well as other
equipment manuals (probes, etc.).
Large-scale and/or long-term monitoring programs such as those envisioned for national
surveys and assessments require a rigorous Quality Assurance (QA) program that can be
implemented consistently by all participants throughout the duration of the monitoring period.
Quality assurance is a required element of all EPA-sponsored studies that involve the collection
of environmental data (USEPA 2000a, 2000b). Field teams will be provided a copy of the
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integrated Quality Assurance Project Plan (QAPP). The QAPP contains more detailed
information regarding QA/QC activities and procedures associated with general field operations,
sample collection, measurement data collection for specific indicators, data reporting activities,
and the information management plan for this project. For more information on the Quality
Assurance procedures, refer to the National Coastal Condition Assessment: Quality Assurance
Project Plan (EPA 841-R-09-004)
Related NCCA documents include the following: 1) National Coastal Condition Assessment:
Quality Assurance Project Plan (EPA 841-R-09-004); 2) National Coastal Condition
Assessment: Site Evaluation Guidelines; and 4) National Coastal Condition Assessment:
Laboratory Methods Manual (EPA 841-R-09-002). These documents are available at:
http://www.epa.gov/owow/monitoring/nationalsurveys.html
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2.0 DAILY OPERATIONS SUMMARY
This Field Operations Manual will be used for sampling at both marine and coastal
freshwater Great Lakes sites. For the most part, the same indicators will be collected, but some
of the sampling will be conducted with different equipment. Additional parameters to be
collected at all Great Lakes sites will include phytoplankton and underwater video of the
substrate. Human health fish tissue samples will be collected at a subset of Great Lakes sites.
This section presents a general overview of the activities that a field team is to conduct during a
typical 1-day sampling visit to a site. General guidelines for recording data using standardized
field data forms and sample labels are also presented. Finally, general safety and health
considerations and guidelines related to field operations are described. Please be sure to fully
know and follow the safety considerations applicable to your organization.
2.1 Sampling Scenario
The field methods for the NCCA are designed to be completed in one field day. Depending
on the time needed for both the sampling and travel for the day, an additional day may be
needed to complete sampling or for pre-departure and post-sampling activities (e.g., cleaning
equipment, repairing gear, shipping samples, and traveling to the next site). Remote sites with
lengthy or difficult approaches may require more time, and field crews will need to plan
accordingly. Conversely, some sites may be in relatively close proximity, allowing multiple sites
to be sampled in a single day.
A field crew will typically consist of three to four people. Each field team should define roles
and responsibilities for each team member to organize field activities efficiently. A minimum of
two people are always required in a boat to execute the sampling activities and to ensure safety.
One crew member is primarily responsible for boat operation and navigation. Any additional
members may assist with the collection of samples or provide logistical support. Daily field
activities may differ depending on whether the team is collecting fish with the use of active
(trawling, seining, hook and line, etc.) or passive (gill net, hoop net, long-lines, etc.) fish
collection methods. Likewise, teams may choose to collect the fish tissue sample on a visit
separate from the collection of water quality samples, sediment and other associated
parameters. Other minor modifications to the sampling scenario may be made by teams;
however the sequence of sampling events presented in Figures 2-1, 2-2 and 2-3 (depending on
the type and timing offish collection) should be adhered to and is based on the need to protect
some types of samples from potential contamination and to minimize holding times once
samples are collected.
Since Enterococcus levels are shown to be highest in the morning before high levels of solar
irradiation, it is recommended that these samples be collected as early in the day as possible
and with minimal disturbance of water and sediment, as long as they are filtered prior to six
hour hold time threshold. Field team should choose the sampling scenario that best fits with
these goals.
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The field team arrives at the site in the early morning to complete the sampling in a single
day. Crew members responsible for collecting water chemistry, sediment grabs and fish tissue
must remember to not apply sunscreen or other chemical contaminants until after the sample is
collected, to avoid compromising the integrity of the sample. The sampling sequence is to:
Verify site as correct location to obtain samples (whole crew);
Make notations of weather, habitat type, presence of submerged aquatic vegetation
(SAV), macroalgae, and debris;
Set net for fish collection (if using passive sampling gear);
Take Secchi disk transparency depth measurements;
Conduct in situ measurements of dissolved oxygen, pH, temperature, and
salinity/conductivity;
Take light attenuation measurements with Photosynthetically Active Radiation (PAR)
meter;
Collect fecal indicator (Enterococci) sample;
Collect water for chemistry and chlorophyll-a;
Collect benthic samples;
Collect sediment samples for chemistry, toxicity, and grain size;
Collect fish tissue samples (note above that if passive sampling gear is used, e.g., a
stationary net, it can be set upon arrival on site);
Filter Enterococci and chlorophyll-a samples;
Collect dissolved nutrients sample (chlorophyll-a filtrate);
Preserve and prepare all samples for shipment;
Review field forms;
Report sampling event; and
Ship time-sensitive samples.
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Arrive on Station
Locate X-site
Verify Sampleability of site
Anchor at X-Site & Record
Coordinates
Record Weather and Water Conditions,
Habitat and Bottom type, and Presence of
Trash, SAV and Macroalgae
Record Depth of Sampling Site
Determine Secchi Disk Depth
Collect Water Column Profile and
Light Measurements
(On both downcast and upcast)
Record video with U/W camera
(Great Lakes Sites only)
Collect Appropriate Water Samples
for Water Chemistry, Chlorophyll-a
(and Phytoplankton in GL sites)
Collect Sediment for Benthic Community
Analysis & Chemistry, Toxicity, and Grain Size
Collect Fish for Tissue Chemistry
Collect Human Health Fish (in GL subset)
Return to X-Site and collect &
Enterococci sample
1 Whole Grab for Benthic
Community Analysis
Additional grab samples of Surficial
Sediment (Homogenized)
TOC
Organics
/ Metals
Toxicity
Grain Size
Filter Enterococci
Sample
_L
Filter Chlorophyll-a
sample
Collect Dissolved
Nutrients Sample
NOTE:
Depending on
crew size and
duties, filtering
may take place
immediately, or at
the end of the
field day.
However, all 4
Enterococci filters
must by
completed and
frozen within 6
hours of
collection.
Figure 2-1. Field Sampling Scenario for Teams Using Active Fishing Methods
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Arrive on Station
Locate X-site
Verify Sampleability of site
Anchor at X-Site & Record
Coordinates
Passive fish collection gear can be
set after site verification to allow
sufficient time to collect fish.
Record Weather and Water Conditions,
Habitat and Bottom type, and Presence of
Trash, SAV and Macroalgae
Record Depth of Sampling Site
Determine Secchi Disk Depth
Collect Water Column Profile and
Light Measurements
(On both downcast and upcast)
Record video with U/W camera
(Great Lakes Sites only)
Collect Appropriate Water Samples
for Enterococci, Water Chemistry,
Chlorophyll-a
(and Phytoplankton in GL sites)
(Collect Enterococci sample first)
Filter Enterococci
Sample
Filter Chlorophyll-a
sample
Collect Dissolved
Nutrients Sample
NOTE:
Depending on
crew size and
duties, filtering
may take place
immediately, or at
the end of the
field day.
However, all 4
Enterococci filters
must by
completed and
frozen within 6
hours of
collection.
Collect Sediment for Benthic Community
Analysis & Chemistry, Toxicity, and Grain Size
1 Whole Grab for Benthic
Community Analysis
Additional grab samples of Surficial
Sediment (Homogenized)
Collect Fish for Tissue Chemistry
Collect Human Health Fish (in GL subset)
TOC
Organics
/ Metals
Toxicity
Grain Size
Figure 2-2. Field Sampling Scenario for Teams Using Passive Fishing Methods
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Arrive on Station
Locate X-site
Verify Sampleability of site
Anchor at X-Site & Record
Coordinates
Record Weather and Water Conditions,
Habitat and Bottom type, and Presence of
Trash, SAV and Macroalgae
Record Depth of Sampling Site
Determine Secchi Disk Depth
Collect Water Column Profile and
Light Measurements
(On both downcast and upcast)
Record video with U/W camera
(Great Lakes Sites only)
Collect Appropriate Water Samples
for Enterococci, Water Chemistry,
Chlorophyll-a
(and Phytoplankton in GL sites)
(Collect Enterococci sample first)
Filter Enterococci
Sample
Filter Chlorophyll-a
sample
Collect Dissolved
Nutrients Sample
Collect Sediment for Benthic Community
Analysis & Chemistry, Toxicity, and Grain Size
NOTE:
Depending on
crew size and
duties, filtering
may take place
immediately, or at
the end of the
field day.
However, all 4
Enterococci filters
must by
completed and
frozen within 6
hours of
collection.
1 Whole Grab for Benthic
Community Analysis
Additional grab samples of Surficial
Sediment (Homogenized)
Organics
/ Metals
Toxicity
Grain Size
Figure 2-3. Field Sampling Scenario for Teams not Collecting Fish for Tissue Chemistry
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2.2 Recording Data and Other Information
All samples need to be identified and tracked, and associated information for each sample
must be recorded. To assist with sample identification and tracking, labels are preprinted and
provided by EPA with sample ID numbers (Figure 2-4).
WATER CHEMISTRY - NOT FILTERED
NCCA10-
./ 72010
999101
NUTRIENTS - FILTERED
NCCA10-
/ /2010
Salinity: %o
999103
SEDIMENT ORGANICS (SEDO)
NCCA10- .
/ /2010
999105
CHLOROPHYLL-a
NCCA10-
./ /2010
Volume Filtered: ml
999102
BENTHOS
NCCA10-
Jar 1 of
999104
/2010
SEDIMENT GRAIN SIZE (SEDG)
NCCA10- .
/ /2010
999106
SEDIMENT TOC(SEDC)
NCCA10-
/ /2010
999107
SEDIMENT TOXICITY (SEDX)
NCCA10-
/ /2010
999108
ECO FISH TISSUE - OUTER BAG
NCCA10-
/ /2010
Genus Species:
Length (mm) Min.: Max.:
999109
ECO FISH TISSUE - INNER BAG .
NCCA10-
./ 72010
Genus Species:
Length (mm) Min.: Max.:
OF
ECO FISH TISSUE - INNER BAG OF
NCCA10-
/ /2010
Genus Species:
Length (mm) Min.: Max.:
999109
999109
ECO FISH TISSUE - INNER BAG OF
NCCA10-
./ 72010
Genus Species:
Length (mm) Min.: Max.:
999109
HUMAN HEALTH FISH TISSUE
NCCAGL10-
/ 72010
Genus Species:
Length (mm):
222001.01
PHYTOPLANKTON
NCCAGL10-
7 72010
999100
Figure 2-4. Example Sample Labels for Sample Tracking and Identification.
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It is imperative that field and sample information be recorded accurately, consistently,
and legibly. The cost of a sampling visit coupled with the short index period severely limits the
ability to resample a site if the initial information recorded was inaccurate or illegible. Illegible or
incorrect information can result in substantially increased time to transfer information from field
forms to the National Aquatic Resource Surveys Surface Water Information Management
System. Guidelines for recording field measurements are presented in Table 2-1.
Table 2-1. Guidelines for Recording Field Measurements and Tracking Information
Activity
Guidelines
Field Measurements
Data Recording
Record measurement values and observations on data forms preprinted on water-
resistant paper.
Use No. 2 pencil only (fine-point indelible markers can be used if necessary) to record
information on forms.
Record data and information using correct format as provided on data forms.
Be sure to accurately record site IDs and sample numbers.
Print legibly (and as large as possible). Clearly distinguish letters from numbers (e.g.,
0 versus O, 2 versus Z, 7 versus T or F, etc.), but do not use slashes.
When recording comments, print or write legibly. Make notations in comments field
only; avoid marginal notes. Be concise, but avoid using abbreviations or
"shorthand" notations. If you run out of space, attach a sheet of paper with the
additional information, rather than trying to squeeze everything into the space
provided on the form.
Data Qualifiers
(Flags)
Use only defined flag codes and record on data form in appropriate field.
K = Measurement not attempted or not recorded.
Q = Failed quality control check; remeasurement not possible.
U = Suspect measurement; remeasurement not possible.
Fn = Miscellaneous flags (n = 1, 2, etc.) assigned by a field team during a
particular sampling visit (also used for qualifying samples).
Explain reason for using each flag in comments section on data form.
Sample Labels
Use adhesive labels with preprinted ID numbers and follow the standard recording
format for each type of sample.
Use a marker to record information on label. Cover the completed label with clear
tape.
Record sample ID number from label and associated collection information on sample
collection form preprinted on water-resistant paper.
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Activity
Guidelines
Sample Collection and Tracking
Sample
Qualifiers
(Flags)
Use only defined flag codes and record on sample collection form in appropriate field.
K = Sample not collected or lost before shipment; resampling not possible.
U = Suspect sample (e.g., possible contamination, does not meet minimum
acceptability requirements, or collected by non-standard procedure).
Fn = Miscellaneous flags (n=1, 2, etc.) assigned by a field team during a
particular sampling visit (also used for field measurements).
Explain reason for using flags in "Comments" on sample collection form.
Review of
Labels and
Data Collection
Forms
Compare information recorded on labels and sample collection form for accuracy
before leaving site.
Review labels and data collection forms for accuracy, completeness, and legibility
before leaving site.
The Field Team Leader must review all labels and data collection forms for
consistency, correctness, and legibility before transfer to the Information
Management Center.
2.3 Safety and Health
Collection and analysis of samples can involve significant risks to personal safety and
health. This section describes recommended training, communications, safety considerations,
safety equipment and facilities, and safety guidelines for field operations.
2.3.1 General Considerations
Important considerations related to field safety are presented in Table 2-2. It is the
responsibility of the crew leader to ensure that the necessary safety courses are taken by all
field personnel and that all safety policies and procedures are followed. Please follow your own
agency's health and safety protocols, or refer to the Health and Safety Guidance for Field
Sampling: National Coastal Condition Assessment (available from the EPA Regional
Coordinator). Additional sources of information regarding safety-related training include the
American Red Cross (2006), the National Institute for Occupational Safety and Health (1981),
and U.S. Coast Guard (1989).
Field crew members should become familiar with the hazards involved with sampling
equipment and establish appropriate safety practices prior to using them. Make sure all
equipment is in safe working condition. Personnel must consider and prepare for hazards
associated with the operation of motor vehicles, boats, winches, tools, and other incidental
equipment. Boat operators should meet any state requirements for boat operation and be
familiar with U.S. Coast Guard rules and regulations for safe boating contained in a pamphlet,
"Federal Requirements for Recreational Boats," available from a local U.S. Coast Guard
Director or Auxiliary or State Boating Official (U.S. Coast Guard, 1989). Personal Flotation
Devices (PFD) must be worn by crew members at all times on the water. All boats with motors
must have fire extinguishers, boat horns, PFDs, and flares or communication devices.
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Table 2-2. General Health and Safety Considerations.
Recommended Training
First aid and cardiopulmonary resuscitation (CPR)
Vehicle safety (e.g., operation of 4-wheel drive vehicles, trailering boats, etc.)
Field safety (weather, personal safety, navigation, site reconnaissance prior to sampling)
Equipment design, operation, and maintenance
Handling of chemicals and other hazardous materials
Communications
Check-in schedule
Sampling itinerary (vehicle used & description, time of departure & return, travel route)
Contacts for police, ambulance, hospitals, fire departments, search and rescue personnel
Emergency services available near each sampling site and base location
Cell (or satellite) phone and VHF radio.
Personal Safety
Field clothing and other protective gear including PFDs for all team members
Medical and personal information (allergies, personal health conditions)
Personal contacts (family, telephone numbers, etc.)
Physical exams and immunizations
A communications plan to address safety and emergency situations is essential. All field
personnel need to be fully aware of all lines of communication. Field personnel should have a
daily check-in procedure for safety. An emergency communications plan should include
contacts for police, ambulance, fire departments, hospitals, and search and rescue personnel.
Proper field clothing should be worn to prevent hypothermia, heat exhaustion, sunstroke,
drowning, or other dangers. Field personnel must be able to swim, and personal flotation
devices must be used. A personal flotation device (PFD) and suitable footwear must be worn at
all times while on board a boat.
Many hazards lie out of sight in the bottoms of coastal areas. Broken glass or sharp pieces
of metal embedded in the substrate can cause serious injury if care is not exercised when
walking or working with the hands in such environments. Infectious agents and toxic substances
that can be absorbed through the skin or inhaled may also be present in the water or sediment.
Personnel who may be exposed to water known or suspected to contain human or animal
wastes that carry causative agents or pathogens must be immunized against tetanus, hepatitis,
typhoid fever, and polio. Biological wastes can also be a threat in the form of viruses, bacteria,
rickettsia, fungi, or parasites.
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2.3.2 Safety Equipment
Appropriate safety apparel such as foul weather gear, safety glasses, etc. must be available
and used when necessary. First aid kits, fire extinguishers, and blankets must be readily
available in the field. Cellular or satellite telephones and/or portable radios should be provided
to field teams working in remote areas in case of an emergency. Supplies (e.g., clean water,
anti-bacterial soap, ethyl alcohol) must be available for cleaning exposed body parts that may
have been contaminated by pollutants in the water.
2.3.3 Safety Guidelines for Field Operations
General safety guidelines for field operations are presented in Table 2-3. Personnel
participating in field activities should be in sound physical condition and have a physical
examination annually or in accordance with organizational requirements. All surface waters and
sediments should be considered potential health hazards due to potential toxic substances or
pathogens. Persons must become familiar with the health hazards associated with using
chemical fixing and/or preserving agents. Chemical wastes can be hazardous due to
flammability, explosiveness, toxicity, causticity, or chemical reactivity. All chemical wastes must
be discarded according to standardized health and hazards procedures (e.g., National Institute
for Occupational Safety and Health [1981]; U.S. EPA [1986]).
During the course of field research activities, field teams may observe violations of
environmental regulations, may discover improperly disposed hazardous materials, or may
observe or be involved with an accidental spill or release of hazardous materials. In such cases
it is important that the proper actions be taken and that field personnel do not expose
themselves to something harmful. The following guidelines should be applied:
First and foremost, protect the health and safety of all personnel. Take necessary steps to
avoid injury or exposure to hazardous materials. If you have been trained to take action such as
cleaning up a minor fuel spill during fueling of a boat, do it. However, you should always err on
the side of personal safety.
Field personnel should never disturb or retrieve improperly disposed hazardous materials
from the field to bring back to a facility for "disposal". To do so may worsen the impact, incur
personal liability for the team members and/or their respective organizations, cause personal
injury, or cause unbudgeted expenditure of time and money for proper treatment and disposal of
the material. Notify the appropriate authorities so they may properly respond to the incident.
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For most environmental incidents, the following emergency telephone numbers should be
provided to all field teams: State or Tribal department of environmental quality or protection,
U.S. Coast Guard, and the U.S. EPA regional office. In the event of a major environmental
incident, the National Response Center may need to be notified at 1-800-424-8802.
Table 2-3. General Safety Guidelines for Field Operations
At least two crew members must be present during all sample collection activities, and no one should
be left alone while out on the water.
Use caution and wear a suitable PFD.
Use caution using the Ponar-type samplers. The jaws are sharp and may close unexpectedly.
Exposure to water and sediments should be minimized as much as possible. Use gloves if necessary,
and clean exposed body parts as soon as possible after contact.
All electrical equipment must bear the approval seal of Underwriters Laboratories and must be
properly grounded to protect against electric shock.
Use appropriate protective equipment (e.g. gloves, safety glasses) when handling and using
hazardous chemicals.
Crews working in areas with poisonous snakes must check with the local Drug and Poison Control
Center for recommendations on what should be done in case of a bite from a poisonous snake.
Any person allergic to bee stings, other insect bites, or plants (i.e., poison ivy, oak, sumac, etc.) must
take proper precautions and have any needed medications handy.
Field personnel should be familiar with the symptoms of hypothermia and know what to do in case
symptoms occur. Hypothermia can kill a person at temperatures much above freezing (up to 10ฐC or
50ฐF) if he or she is exposed to wind or becomes wet. Immersion in the cool waters experienced
during the summer along most of the coast and Great Lakes can also rapidly result in hypothermia.
Field personnel should be familiar with the symptoms of heat/sun stroke and be prepared to move a
suffering individual into cooler surroundings and hydrate immediately.
Handle and dispose of chemical wastes properly. Do not dispose of any chemicals in the field.
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3.0 BASE SITE ACTIVITIES
Field teams conduct a number of activities at their base site (i.e. office or laboratory,
camping site, or motel). These include tasks that must be completed both before departure to
the site and after return from the field (Figure 3-1). Close attention to these activities is required
to ensure that the field teams know: 1) where they are going, 2) that access is permissible and
possible; 3) that equipment and supplies are available and in good working order to complete
the sampling effort; and 4) that samples are packed and shipped appropriately.
PREDEPARTURE ACTIVITIES
Crew Members
In stru m ent c li ec ks & c a librati o n
Equipments supplies
Whole Crew preparation
* Site verification
V _
Team Leader
Prepa re cl a ily itin era ry
Team Leader
Review forms and labels
File status report by email to the tracking team
email addresses
Crew Members
Filter, preserves, in sped samples
CI ea n boats with 1-10% blea c h so lution a n d
perform safety checks (when trailering between
one water body to distinctly different water body)
Clean (and repair, if needed) sampling gear
* Charge or replace batteries
Refuel vehicle and boat
* Obtain ice and other consumable supplies as
needed
Pa c ka ge a n d sh ip sa mples & data fo rms J
Figure 3-1. Overview of Base Site Activities.
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3.1 Predeparture Activities
Predeparture activities include the development of a daily itinerary, instrument checks and
calibration, and equipment and supply preparation. Procedures for these activities are described
in the following sections.
3.1.1 Daily Itineraries
The Field Team Leaders are responsible for developing daily itineraries. This entails
compiling maps, navigational charts, contact information, copies of permission letters, permits,
access instructions, location of FedEx offices, and location of hospitals or other emergency
services (a "site packet"). Additional activities include confirming the best access routes, calling
the landowners or local contacts, confirming lodging plans, and coordinating rendezvous
locations with individuals who must meet with field teams prior to accessing a site. Also, the
Leader should identify appropriate boat ramps or marinas, and gas docks. If the crew is
planning a multiple day/multiple site trip, information for each day and site must be developed.
Field Team Leaders should call the Site Kit Coordinator or Field Logistics Coordinator at
least two weeks in advance to request site kits based on the upcoming schedule. Changes in
the itinerary during the week, such as canceling a sampling day, must be relayed by the crew
leader to the Field Logistics Coordinator as soon as possible.
3.1.2 Instrument Checks and Calibration
Each field team must test and calibrate instruments prior to sampling. Calibration can be
conducted prior to departure for the site or at the site, with the exception of dissolved oxygen
(DO) calibration. DO meters should be calibrated at the site. Field instruments include a global
positioning system (GPS) receiver, a Photosynthetically Active Radiation (PAR) meter, and a
multiprobe unit for measuring DO, pH, temperature, salinity (marine sites) and conductivity
(freshwater sites). Field teams should have access to backup instruments if any instruments fail
the manufacturer performance tests or calibrations. Prior to departure, field teams must:
Turn on the GPS receiver and check the batteries if using hand-held GPS unit. Replace
batteries immediately if a battery warning is displayed. Otherwise, the GPS is installed
on the boat and runs off of the boat electrical system.
Test and calibrate the multi-probe meter. Each field team should have a copy of the
manufacturer's calibration and maintenance procedures. All meters should be calibrated
according to manufacturer specifications provided along with the meter. Once a week,
crews should check their multiprobe against the provided Quality Check Solution. This
QCS is provided to all crews in their base kits and is used to check pH and conductivity
measurements.
Ensure that the PAR meter's handheld display unit has fresh batteries, that the unit is
functioning properly, and that the correct calibration factors are entered for each probe.
These factors are supplied by the manufacturer and are specific to each individual
probe. PAR sensors require no field calibration, however, they should be returned to the
manufacturer at least every 2 years for calibration. Procedures for the initial setup of the
LI-COR LI-1400 Datalogger is presented in Table 3-1. These steps can be used to
verify the setup of the unit, or to enter coefficient values should a new sensor need to be
installed.
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For teams operating in the Great Lakes, ensure that the underwater video system's
battery is charged and all components are hooked up correctly. Ensure that the
attached GPS is set up to output information to the GPS overlay (this will be done prior
to shipment of the system to field crews, but should a crew need to verify setup, refer to
Section 5.5.3).
Table 3-1. Initial Setup Procedures for LI-COR LI-1400 Datalogger
LI-COR systems received from GLEC will have been configured for use already and will be ready for
sampling, these instructions will be for future reference.
The following example demonstrates how you can configure the LI-1400 with the instrument keypad to
view or log instantaneous data from a single LI-190SA Quantum Sensor.
Example 1a. Configure channel 11 fora LI-COR LI-190SA Quantum Sensor whose calibration multiplier is
-125.0[jmols-1m-2/ijAmp (Each sensor has a unique multiplier value supplied from the factory)
1. Connect the Quantum LI-190 sensorto the BNC connector on top of the LI-1400 labeled 11.
2. Turn on the LI-1400 meter.
3. Press the Setup key.
4. Use the left or right arrow keys to navigate to "SETUP CHANNELS".
5. Press the Enter key to begin the sensor setup.
6. Use the left or right arrow keys to navigate to "M=Light", press Enter".
7. Using the Shift key and the number/ letter keys, type a description for this channel.
This description can be anything such as QUANTUM to describe the type of sensor, orAMB to
describe what the reading will be used for in the NCCA sampling.
8. Press the down arrow key to enter the multiplier.
Use the Multiplier value found on the Certificate of Calibration that came with your sensors. There
should be a unique certificate and calibration multiplier value for each sensor.
9. Press the down arrow key; enter the unit label. Type UM for the label.
10. Press the down arrow key; select "1 sec" to have instantaneous values displayed.
The running average parameter will not be used, but could be set here to any desired value.
11. Press the down arrow key; select "Log Routin=none"
12. The remaining options do not need to be set as they apply only when using a Log Routine.
13. Repeat this entire procedure for "!2=Light" to setup the underwater sensor.
3.1.3 Equipment and Supply Preparation
Field teams must check the inventory of supplies and equipment prior to departure using the
equipment and supplies checklists provided in Appendix A; use of the lists is mandatory. Obtain
sufficient wet and dry ice for sample preservation and storage. Pack meters, probes, and
sampling gear in such a way as to minimize physical shock and vibration during transport. Pack
stock solutions as described in Table 3-2. Follow the regulations of the Occupational Safety and
Health Administration (OSHA).
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Table 3-2. Stock Solutions, Uses, and Methods for Preparation.
Solution
Bleach (1-10%)
Quality Check
Solution for multi-
probe meter
Buffered Formalin
Lugol's Solution
Use
Clean nets, gear, and inside of boat
QCS for pH and conductivity calibration
Preserve benthic samples
Preserve phytoplankton samples
(Great Lakes sites only)
Preparation
Add 10 -100 ml bleach to 1 L
distilled water.
None (included in base kits)
Add % teaspoon Rose Bengal
crystals and 8 tablespoons Borax to
2 gallons 100% Formalin solution
None (included in GL base kits)
Site kits of consumable supplies for each sampling site will be delivered based on the
schedule each crew provides prior to the sampling season. Field crew leaders MUST provide
a schedule in order to receive the site kits and must call the Field Logistics Coordinator
two weeks prior to sampling. Field crew leaders involved with Great Lakes human health fish
sampling must specifically request a human health fish tissue supply kit for those sites from the
Great Lakes Human Health Fish Tissue Field Kit Coordinator. Please note, field kits for all sites
cannot be provided at the beginning of the field season but will be sent out as requested
throughout the index period. If your schedule changes, report the change as soon as possible to
the Field Logistics Coordinator. The site kit will include data forms, labels, sample jars, bottles
and other supplies (see complete list in Appendix A). The teams must inventory these site kits
before departure to ensure that all supplies are included. If any items are missing or incorrect,
crews must request these supplies from the Site Kit Coordinator as soon as possible so that the
supplies are received prior to departure. Container labels should not be covered with clear tape
until all information is completed during sampling at the site. Store extra sampling site kits in the
vehicles in case of loss, damage, etc. Inventory these extra site kits prior to each site visit to
ensure sufficient back-up supplies are available.
3.1.4 Chill Enterococci Filter Extraction Tubes
In preparation for later filtering, remove Enterococci filter extraction tubes with beads from
the filter kit provided in the site kit and place on dry ice.
3.2 Post Sampling Activities
Upon return to the launching location after sampling, the team must perform a post-
measurement calibration check of the multi-probe meter, review all completed data forms and
labels for accuracy, completeness, and legibility and make a final inspection of samples. If
obtainable samples are missing, the site should be rescheduled for complete sampling. Other
post sampling activities include: inspection and cleaning of sampling equipment, supply
inventory, sample and data form shipment, and communications.
3.2.1 Post-measurement Calibration Check of Multi-probe Meter
After all in situ measurements have been completed for the sampling day, the team must
perform a post-measurement calibration check of the instrument to detect any drift from the pH
and conductivity calibration values. To do this, measure the pH and conductivity of the
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respective calibration standards that were used earlier in the day to calibrate the instrument.
Record these values on the Field Measurement Form. If significant drift is detected, it may
indicate that the meter is in need of service.
3.2.2 Review Data Forms and Labels
The field crew leader is ultimately responsible for reviewing all data forms and labels for
accuracy, completeness, and legibility. Ensure that written comments use no "shorthand" or
abbreviations. The data forms must be thoroughly reviewed. If information is missing from the
forms or labels, the Field Team Leader is to provide the missing information. Upon completing
the review, the field crew leader must initial the field forms to indicate that they are ready to be
sent to the Information Management Center. Each sample label must also be checked for
accuracy, completeness, and legibility. The field crew leader must cross-check the sample
numbers on the labels with those recorded on the data forms and tracking forms.
3.2.3 Inspect and Prepare Samples
All samples need to be inspected and appropriately preserved and packaged for transport.
Check that all samples are labeled, and all labels are completely filled in. Check that each label
is covered with clear plastic tape. Check the integrity of each sample container, and be sure
there are no leaks. Make sure that all sample containers are properly sealed. Make sure that all
sample containers are properly preserved for storage or immediate shipment.
3.2.4 Equipment Cleanup and Check
All equipment and gear must be cleaned and disinfected when traveling over land between
distinctively different sites to reduce the risk of transferring nuisance species and pathogens.
Species of primary concern in the U.S. include zebra mussels (Dreissena polymorpha), mitten
crabs (Eriocheirsinensis), and Eurasian ruffe (Gymnocephalus ceinuus). Field crews must be
aware of regional species of concern, and take appropriate precautions to avoid transfer of
these species. There are several online resources regarding invasive species, including general
information about aquatic nuisance species available from the Aquatic Nuisance Species Task
Force (http://www.anstaskforce.gov). General information about freshwater invasive species is
available from the U.S. Geological Survey Nonindigenous Aquatic Species website
(http://nas.er.usqs.qov), the Protect Your Waters website that is co-sponsored by the U.S. Fish
and Wildlife Service (http://www.protectyourwaters.net/hitchhikers), and the Sea Grant Program
(http://www.sgnis.org). In the Great Lakes, Viral Hemorrhagic Septicemia (VMS) is a deadly fish
virus and an invasive species that is threatening Great Lakes fish. VMS was diagnosed for the
first time ever in the Great Lakes as the cause of large fish kills in lakes Huron, St. Clair, Erie,
Ontario, and the St. Lawrence River in 2005 and 2006.
Handle and dispose of disinfectant solutions properly, and take care to avoid damage to
lawns or other property. Table 3-3 describes equipment care. Inspect all equipment, including
nets, boat, and trailer, and clean off any plant and animal material. Prior to leaving a site, drain all
bilge water and live wells in the boat. Inspect, clean, and handpick plant and animal remains from
vehicle, boat, motor, and trailer. Before moving to the next site, if a commercial car wash facility is
available, wash vehicle, boat, and trailer and thoroughly clean (hot water pressurized rinse-no
soap). Rinse equipment and boat with 1% -10% bleach solution to prevent the spread of exotics.
For specific techniques to disinfect boats and gear in the Great Lakes, please see Appendix C.
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Table 3-3. Postsampling Equipment Care
1. Clean for biological contaminants.
Prior to departing site, drain all bilge water from the boat.
Inspect motor, boat, trailer, sampling gear, foul weather gear, boots, etc. for evidence of mud,
snails, plant fragments, algae, animal remains, or debris, and remove using brushes or other tools.
At the base location, inspect and rinse seines, dip nets, sieves, foul weather gear, and boots with
water and dry. Use one of the procedures below to disinfect gear if necessary.
Additional precautions to prevent transfer of Whirling Disease spores, New Zealand mudsnails, and
amphibian chytrid fungus is important for Great Lakes sites. Before visiting the site, research the site and
determine if it is in an area where whirling disease, New Zealand mud snails, or chytrid fungus are known
to exist. Contact the local State fishery biologist to confirm the existence or absence of these organisms.
If the site is listed as "positive" for any of the organisms, or no information is available, avoid using
felt-soled wading boots, and, after sampling, disinfect all fish and benthos sampling gear and
other equipment that came into contact with water or sediments (i.e., waders, boots, etc.) by one
of the following procedures:
Option A:
1. Soak gear in a 10% household bleach solution for at least 10 minutes, or wipe or spray on
a 50% household bleach solution and let stand for 5 minutes
2. Rinse with deionized water (do not use sea or lake water), and remove remaining debris
3. Place gear in a freezer overnight, soak in a 50% solution of Formula 409ฎ antibacterial
cleaner for at least 10 minutes or soak gear in 120ฐF (49ฐC) water for at least 1 minute.
4. Dry gear in direct sunlight (at least 84 ฐF) for at least 4 hours.
Option B:
1. Soak gear in a solution of Sparquatฎ (4-6 oz. per gallon of water) for at least 10 minutes
(Sparquat is especially effective at inactivating whirling disease spores).
2. Place gear in a freezer overnight or soak in 120ฐF (49ฐC) water for at least 1 min.
3. Dry gear in direct sunlight (at least 84 ฐF) for at least 4 hours.
2. Clean and dry other equipment prior to storage.
Rinse coolers with water to clean off any dirt or debris on the outside and inside.
Make sure water quality meter probes are rinsed with deionized water and stored moist.
Rinse all beakers used to collect water chemistry samples three times with deionized water. Place
sampling equipment in a clean location for use at the next site.
Check nets for holes and repair or locate replacements.
3. Inventory equipment and supply needs and relay orders to the Field Logistics Coordinator.
4. Remove GPS and multi-probe meter, and set up for predeparture checks and calibration. Examine the
oxygen membranes for cracks, wrinkles, or bubbles. Replace if necessary, allowing sufficient time for
equilibration.
5. Recharge/replace batteries as necessary.
6. Replenish fuel and oil;
7. If a commercial car wash facility is available, thoroughly clean vehicle and boat (hot water pressurized
rinseno soap).
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3.2.5 Shipment of Samples and Forms
3.2.5.1 Samples
The field team must ship or deliver time-sensitive samples (i.e., water chemistry, chlorophyll-
a, sediment-grain size, sediment-TOC, and dissolved nutrients) to the appropriate analytical
laboratory (WRS Corvallis) as soon as possible after collection. Other samples (see Appendix
D) may be shipped or delivered in batches provided they can be adequately preserved. Batched
samples should be shipped every two weeks. Field teams are to fill out one sample tracking
form for each sample shipment. On each sample tracking form, the following information must
be recorded:
Airbill or package tracking number;
Date sample(s) were sent;
Site ID where each sample was collected;
Sample type code:
CHEM - Water Chemistry
CHLA - Chlorophyll-a
NUTS - Dissolved Nutrients
ENTE - Enterococci
FTIS - Fish Tissue Composite
PACK - Field Form Packet
HTIS - Human Health Fish Tissue
(Great Lakes subset only)
BENT - Benthos Grab
SEDX - Sediment Toxicity
SEDG - Sediment Grain Size
SEDO - Sediment Organics/Metals
SEDC - Sediment TOC
PHYT - Phytoplankton (Great Lakes Only)
UVID - Underwater Video
(Great Lakes Only)
Date when the sample(s) was collected (1st day if sampling took >1 day);
Site visit number (e.g., 1 for first visit, 2 for re-visit);
Sampler name and contact information;
Sample ID number encoded on label;
Number of containers for each sample;
Destination lab; and
Any additional comments.
It is important that the correct tracking form (see Section 3.2.6.2) be completed, placed into
a waterproof plastic bag, and secured inside the shipping container (e.g., taped to the inside top
of the coolers). Detailed sample shipping instructions are presented in Appendix D.
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3.2.5.2 Field Forms
After checking the Field Forms for completeness and accuracy, the Field Crew Leader will
make copies of all Field Forms and retain the copies. The original forms will be mailed to
Marlys Cappaert in the FedEx envelope provided in the site kit. A pre-addressed airbill will
be provided. The original forms must be sent because they are printed specifically to be used in
a scanner for automated data entry. Field forms may be retained and mailed in batches
throughout the field season (every 2 weeks) when it is convenient to make the copies. All field
forms must be turned in within 2 weeks of completing sampling. A tracking form will be
submitted with each shipment of data forms. The data forms will be tracked in the same
manner as all other samples.
3.2.6 Status Reports and Communications
3.2.6.1 Sample Status Report
After each site visit, the field crew leader must submit a sample status report to the
Information Management Coordinator to report the site visit and indicate which samples were
collected and their respective sample ID numbers. This status report must be submitted before
the time sensitive samples are due to arrive at the lab. This ensures that the laboratory is
prepared to receive the samples and will help track down the samples should they become lost
in transit. The field crew must also ship all time sensitive samples such that they will arrive at
the WRS lab within 48 hours of collection. This requires the samples be sent by Priority
Overnight shipping the same day as collection, or at the latest, the following day. A tracking
form must accompany every sample shipment.
For convenience, the WRS sample tracking form and the site status report are incorporated
into a single form called the Tracking and Sample Status form (Figure 3-2). Teams have the
option of filling this form out digitally using Microsoft Word or manually filling out the scannable
version of the form that is provided in the set of field forms. See below for more information on
the form submission options available to crews.
If the crew visits a site with the intention of sampling, but determines the site to be
unsampleable (either temporarily or permanently), the site status portion of the form needs to be
completed and submitted, but the WRS tracking portion of the form can remain blank.
3.2.6.2 Tracking Forms
Regardless of the type of sample being shipped, a tracking form must be completed for
every shipment and a copy must be placed inside the container with the samples (typically
sealed in a plastic bag and taped to the inside of the cooler lid). Again, teams have the option of
filling this form out digitally using Microsoft Word or manually filling out the scannable version of
the form that is provided in the set of field forms. A copy of the tracking form must also be
submitted to the Information Management Coordinator before the samples are due to arrive at
the lab. See below for more information on the form submission options available to crews.
Samples Shipped Immediately
For time sensitive samples, fill out the Tracking and Sample Status form, the lower portion
has the sample ID numbers for each sample being sent.
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Batched Samples
Samples that are less time sensitive can be held for up to 2 weeks and sent to the
appropriate lab in batches. Fill out a Batched Samples Tracking Form (Figure 3-3) with the
sample types and sample ID numbers. Use a separate form for each lab.
This form must be filled out and submitted:
when samples are brought into your lab or holding facility, and
then again when the samples are shipped.
Fish Tissue and Human Health Fish Tissue Samples
Separate tracking forms will be completed and submitted for each fish tissue sample.
Separate tracking forms are used for the ecological fish tissue collections (Figure 3-4) and
human health fish tissue collections (Figure 3-5). Human health fish tissue samples will be
collected at a subset of Great Lakes sites only.
3.2.6.3 Methods of Communication (in order of preference)
1) E-mail submission: Electronic versions of the Tracking and Sample
Status form and the Batched Samples Tracking form will be emailed to
the field crew leaders after their training session. Complete the Tracking
and Sample Status report form for each site, even sites that are visited
but not sampled, and email the form to sampletracking@epa.gov. This
email will go to both the Information Management Coordinator and the
Field Logistics Coordinator.
You must follow a standardized naming convention when naming the
electronic Tracking and Sample Status report files. The naming
convention for this form is:
"labid_siteid_datecollected.doc:"
ex.WRS_NCCA10OR123_06_28_2010.doc
For batch samples, the naming convention is:
"BR_labid_siteid_datecollected.doc:"
ex. BR_GLEC_NCCA10OR123_06_28_2010.doc (in this case,
the site id and date collected will refer to the first sample on the
page)
Be sure to print a copy of the tracking form to be placed inside the
container with the samples prior to sealing the container for shipping.
2) Fax Submission: If you are not able to email the electronic forms, the
forms can be faxed on a non-voice over internet phone (VOIP) fax
machine. This could be a printed version of your electronic form or a hand
written copy of the scannable version of the form that is provided in the
set of field forms.
The fax number for tracking form submission is 541-754-4637
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3) Voice Submission: If neither emailing nor faxing the forms is feasible,
the team leader may call into the number provided on the bottom of the
Tracking and Sample Status form (read the ENTIRE form to the voice
mail machine. It is extremely important that all information from the form
is transferred; do not leave any information out of your message).
The voice number for tracking form submission is 541-754-4663
Information Management Coordinator
Marlys Cappaert 541-754-4467 Cappaert.Marlys@epamail.epa.gov
Sample Tracking email submission: sampletracking@epa.gov
Sample Tracking fax submission: 541-754-4637
Sample Tracking voice submission: 541-754-4663
Primary Field Logistics Coordinator
Jennifer Under 410-356-8993 Jennifer.Linder@tetratech.com
Alternate Field Logistics Coordinator
Chris Turner 715-829-3737 cturner@glec.com
Other Information
It is very important to complete the sample status report immediately after every sampling
event. This will enable the Field Logistics Coordinator to track sampling progress. More
importantly, it will enable the Information Management Center to track which samples were
collected at each site, and to immediately track the shipment of the time-sensitive samples that
will be shipped after each sampling event.
The field crews should call or email the Field Logistics Coordinator to report any problems
encountered. The Field Logistics Coordinator monitors all aspects of field sampling activities.
The Field Logistics Coordinator and Information Management Coordinator will contact the EPA
Headquarters Coordinator regularly to provide regional updates throughout the sampling period.
The EPA Headquarters Coordinator will maintain a database of all sampling activities and
reconnaissance information.
The EPA Regional Coordinator serves as the central point of contact for information
exchange among field teams, the management and QA staffs, the information management
team, and the public. A list of EPA Regional Coordinators and their contact information can be
found at the beginning of this manual on page ix.
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Page 28
NCCA2010 TRACKING AND SAMPLE STATUS -WRS
SITE ID: NCCA10-
SENTBY:
Visit #: O1 O2 i
SENDER PHONE:
Date Collected: / / 2 0 1 0
State of Site Location: TEAM: DATE SENT: / / 2 0 1 0
SHIPPED O FedEx OUPS O Hand Delivery
BY -. _ . AIRBILL/TRACKING
O Other: NUMBER:
SITE STATUS
SAMPLEABLE NOT SAMPLEABLE NO AC
O Marine Q Shallow O Access
O Great Lakes Q Unsafe Olnacce
Temporarily O Map Error O Temp I
Not Sampleable oother
O Other (Explain in Status
(Explain in Status Comments)
Comments)
SAM RLE STATUS
O No Samples Collected
CESS Mark the samples that were collected during this site visit:
i Denied O Water Chem (CHEM) O Sediment TOC (SEDC)
ssible O Chlorophyll-a (CHLA) O Sediment Grain (SEDG)
naccessible O Nutrients (NUTS) O Benthos Grab (BENT)
O Sediment Organics (SEDO)O Enterococci (ENTE)
O Sediment Toxicity (SEDX) O Fish Tissue (FTIS)
O Human Hej
OPhytoplankI
(Great Lakes Only) !
ilth Fish Tissue (HTIS) O Video Card (UVID) I
on (PHYT)
Status Comments
Sample ID Sample Type Com me
CHEM
CHLA
NUTS
SEDC
SEDG
Sample Types Condition Codes
Filled in by recipient
CHEM - Water chem stry
CHLA - Chlorophyll-a C- Cracked jar
NUTS - Nutrients F = Frozen
SEDC - Sediment TOC L = Leaking
SEDG - Sediment Grain Size ML = Missing label
NP = Not preserved
W =Warm
OK = Sample OK
T= Thawed
nts
Chain of Custody
Filled in by recipient
Date Rece ved:
Received by:
Contact Information
Tracking Assistance:
Marlys Cappaert Michelle Gover
541-754-4467 541-754-4793
Lab:
Attn: Phil Monaco, Dynamac
c/oU.S. EPA
1350 Goodnight Ave
Corvallis, OR 97333
PH: 541-754-4720
monaco.phil@epamail.epa.gov
FAX THIS FORM TO 541-754-4637
OR READ TRACKING INFO TO VOICE MESSAGE CENTER:
04/22/2010 NCCA Tracking - WRS 541-754-4663
8299111157
Figure 3-2. Example Tracking and Sample Status Form
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NCCA 2010 TRACKING - BATCHED SAMPLES
SENDER
SENT BY: PHONE:
Shipped o FedEx OUPS O Hand Delivery DATE SHIPPED:
AIRBILL/TRACKING
NUMBER:
O Held at address:
Site ID
NCCA10-
NCCA10-
NCCA10-
NCCA10-
NCCA10-
NCCA10-
NCCA10-
NCCA10-
NCCA10-
NCCA10-
NCCA10-
NCCA10-
NCCA10-
NCCA10-
NCCA10-
NCCA10-
Date Sample Collected
MM/DD/YYYY
Visit
01
o?
01
02
01
02
01
o?
01
02
01
o?
01
02
01
02
01
o?
01
02
01
o?
01
o?
01
o?
01
o?
01
02
01
02
Sample ID
STATE OF
SITE LOCATION: TEAM:
/ / 2 0 1 0
Sam pie Type
Lab Chain of Custody
QBENTHIC LAB
QGLEC
QMED
QNERL- N CHELMSFORD, yA
QTETRATECH
Q WED - CORVALLIS, OR
O OTHER
Filled in by recipient
Date Received:
/ /
Received by:
# of
Containers
Comments
Cond,
Code
Sample Types Condition Codes
Filled in by recipient
BENT - Benthos Grab
ENTE - Enterococci c = Cracked jar
SEDX - Sediment Toxicity
SEDO - Sediment Organics/Metais F ~ Frozen
PHYT - Phytoplankton (Great Lakes L = Leaking
Only) ML = Missing label
PACK -Field Form Packet NP = Not preserved
W = Warm
Tracking Assistance: OK = SamP|e OK
.. , _ . ซ-,,! T = Thawed
Marly s Cappaert Michelle Cover
541-754-4467
541-754-4793
FAX THIS FORM TO 541-754-4637 OR READ TRACKING INFO TO VOICE MESSAGE CENTER: 541-754-4663
04/22/2010 NCCA Tracking - Batch
1059022391
Figure 3-3. Example Batched Samples Tracking Form
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NCCA 2010 ECO FISH TISSUE TRACKING
SITE ID: NCCA10- VISIT: Q1 O2
DATE COLLECTED: f / 2 0 1 0
SENT BY: SENDER PHONE:
STATE OF SITE LOCATION: TEAM:
SHIPPED BY: O FedEx O Other:
AIRBILL/TRACKING
NUMBER:
DATE SHIPPED: / / 2 0 1 0
SAMPLE ID
Condition
Genus Species Total Length (mm) Comments code
.01
.02
.03
.04
.05
.06
.07
.08
.09
.10
.11
.12
.13
.14
.15
.16
.17
.18
.19
.20
Filled in by recipient
Condition Codes Chain of Custody
L = Leaking Date Received:
ML = Missing label / /
NP = Not preserved
W = Warm Received by:
OK = Sample OK
Contact Information
Tracking Assistance: Lab Contact:
Marlys Cappaert ???
541-754-4467 PH: ???
Michelle Cover
541-754-4793
04/22/2010 NCCA Tracking - Fish Tissue
3080542800
Figure 3-4. Example Ecological Fish Tissue Tracking Form
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NCCA 2010 HUMAN HEALTH FISH TISSUE TRACKING
SITE ID: NCCAGL10- VISIT: Q1 O2
DATE COLLECTED: / / 2 0 1 0
SENT BY: SENDER PHONE:
STATE OF SITE LOCATION: TEAM:
SHIPPED BY: O FedEx O Other:
AIRBILL/TRACKING DATE SHIPPED: / / 2 0 1
UIIMRFD- , , ,
0
SAMPLE ID
Condition
Genus Species Total Length (mm) Comments code
.01
.02
.03
.04
.05
Filled in by recipient
Condition Codes Chain of Custody
L = Leaking Date Received:
ML = Missing label / /
NH - Not preserved
W = Warm Received by:
OK = Sample OK
Contact Information
Tracking Assistance: Lab Contact:
Marlys Cappaert Harry (Chip) McCarty
541-754-4467 703-461-2392
Michelle Cover Carolina Gallardo
541-754.4793 410-356-8993
04/22/2010 NCCA Tracking - Human Health Fish Tissue
5582497224
Figure 3-5. Example Human Health Fish Tissue Tracking Form
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Page 32
4.0INITIAL SITE PROCEDURES
When you arrive at a site, you must first confirm you are at the correct site, and then
determine if the site meets the criteria for sampling and data collection activities (see Site
Evaluation Guidelines). Inspect the site for appropriate access, safety, and general conditions to
determine if the site can be sampled within the swing of the boat while anchored.
Please remember that crew members responsible for collecting water chemistry, sediment
and fish tissue samples must not apply sunscreen or other chemical contaminants until after the
sample is collected.
4.1 Site Verification Activities
4.1.1 Locating the X-Site
Base site sampling points were chosen using a Generalized Random Tessellation Stratified
(GRTS) survey design, which is a stratified design with equal probability of selection. Each point
is referred to as the "X-site." The X-site is the point that determines the location at which
samples are taken. The latitude/longitude of the X-site is listed on the site spreadsheet that was
distributed by the EPA Regional Coordinators. Table 4-1 provides a list of equipment and
supplies necessary for locating and verifying the sampling site.
4.1.2 Target population
The target population for the estuarine resources consists of all coastal waters of the
conterminous United States from the head-of-salt to confluence with the ocean, including inland
waterways, tidal rivers and creeks, lagoons, fjords, bays, and major embayments such as
Florida Bay and Cape Cod Bay (see Figure 4-1 and 4-2). For the purposes of this study, the
head of salt is generally defined as < 0.05 psu (ppt) and represents the landward/upstream
boundary. The seaward boundary extends out to where an imaginary straight-line intersecting
two land features would fully enclose a body of coastal water. All waters within the enclosed
area are defined as estuarine, regardless of depth or salinity.
The target population for the Great Lakes encompasses all near-shore waters. The near
shore zone is defined as the region from the shoreline to 30m in depth constrained to a
maximum of 5 km from shore. The Great Lakes include Lake Superior, Lake Michigan, Lake
Huron, Lake Erie, and Lake Ontario. The National Aquatic Survey will be restricted to the United
States portion.
Table 4-1. Equipment and Supplies List for Site Verification.
For locating and
verifying site
Sampling permit and landowner access (if required)
Field Operations Manual and/or laminated quick reference guide
Site packet, including access information, site spreadsheet with map
coordinates, navigational charts with "X-site" marked
NCCA Fact Sheets for public outreach
GPS unit (preferably one capable of recording waypoints) with manual,
reference card, extra battery pack
For recording
measurements
Clipboard
#2 pencils
Site Verification Form
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Page 33
Legend
I I Estuarine System
Law
Marine Nearshore Coastal Waters
Legend
| Estuarine System
Land
| Marine Nearshore coastal waterc
Figure 4-1: Example of an Estuarine System
Comprised of an Embayment plus a Complex of
Bays and Tidal Rivers and Creeks.
Figure 4-2: Example of an Inter-coastal Estuarine
System.
4.1.3 Site Verification
Identify the X-site using GPS and navigate to the location within 0.02 nautical miles (nm)
(ฑ37 meters) of the given coordinates. Record the coordinates from the EPA-provided site list
on the field verification form as the "target" coordinates. Record the actual coordinates of the
vessel after anchorage on the field verification form as the "actual" coordinates. Samples
should be taken as close to these coordinates (actual X-site) as possible. Teams are expected
to collect all samples within a circle of 0.02 nm radius around the X-site (see Section 4.1.6
regarding secondary collection areas for sediment). This distance should account for typical
"anchor swing" of the sampling vessel. It is recommended that teams create a GPS waypoint
shortly after anchoring the boat and periodically consult the GPS during sampling to ensure that
the sampling vessel has not drifted away from the X-site due to anchor drag.
The field team must verify that the site is correctly located. Sampling site verification is
based on map coordinates and locational data from the GPS. Record locational coordinates for
the site on the Site Verification Form. Latitude and longitude are required for all sampled sites.
Include the number of satellites fixed (< 3 or > 4), and the GPS datum used (e.g., WGS 84) for
QA purposes. Compare the map coordinates given on the coastal survey spreadsheet for the
targeted sampling point with the GPS coordinates displayed for the sampling site, and check to
see if the two sets of coordinates are within 0.004167 decimal degrees of latitude and longitude.
This distance is approximately equal to the precision of the GPS receiver without differential
correction of the position fix. This is the desired level of precision.
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Size and shape of the waterbody in which the X-site resides will vary depending on
coastal morphology. While site depth or salinity should not generally be a factor for abandoning
a planned sampling site, there are some points that a field crew may consider in order to
determine if an X-site meets the operational definition of an estuary in marine environments, or
lacustrine and near shore coastal waters in the Great Lakes:
Access to open water;
Navigable using a shallow-draw boat. Typically this means that the depth of the X-Site is
generally > 1 meter. Actual depth determinate, however, may be based on the vessel
and sampling equipment used, and wave action at the site.
If the specific site does not fit this definition and every attempt to relocate a site within the
margin provided (see Section 4.1.4) has been made, complete the appropriate "Non-
Sampleable-Permanent" category on the Site Verification Form and provide an explanation for
not sampling the site in the comments section of the form. Add any additional explanation as
required. (For complete details on the site evaluation process, refer to the Site Evaluation
Guidelines).
If the site is non-sampleable or inaccessible, no further sampling activities are conducted.
Replace the site with the next oversample site on the estuary/state list. Notify the EPA Regional
Coordinator and Field Logistics Coordinator (Section 3.2.6) that the site was replaced and
submit the verification form to the Information Management Coordinator. Refer to the See Site
Evaluation Guidelines for further information regarding the replacement of sites.
If the site is sampleable, record the sampling status and pertinent site verification
information on the Site Verification Form (Figure 4-3) including the time of arrival at the X-site
and water depth. Make sure an accurate depth reading is taken at the site to ensure the depth is
adequate to conduct sampling. Refer to Table 4-2 for detailed information regarding the site
verification process.
Record the names of the field team on the back of the Site Verification Form (Figure 4-4).
Also create a general site sketch of the area. Include the relative locations of the shoreline,
launch point, X-site, fish collection location, and sediment location if different than the X-site
(see Section 4.1.6). Include any other specific attributes of the site that may be important during
the data processing portion of the assessment. A printed or copied section of a map with the
pertinent information may be submitted in place of the site sketch.
4.1.4 Site Relocation
For relocation situations, every attempt should be made to relocate a site within a 0.02 nm
(-37 m) radius of the intended location. A guideline for the relocation effort follows:
The field crew leader should choose a specific compass heading (e.g., north, south,
east, west) and slowly motor the vessel in that direction for approximately 15-20 meters.
Assess the relocated site using the Site Verification guidelines given above. Should the
relocated site fail to meet the operational definition "sampleable", then this process may
be continued using the same heading out to the 37 meter mark or using a new heading
until an acceptable sampling location is found. If after a sufficient amount of effort is
expended and no suitable site is found, then the determination may be made that the
site is unsampleable.
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page 35
4.1.5 Sample Collection
While the field crew should make every attempt to collect all samples, there will be some
circumstances that will prevent this from happening. Following is a guideline for prioritizing
sample collection at each site and a "check-list" for determining sample completion when site
conditions limit full completion of the standard sampling protocol:
In-situ water measurements and water samples are expected to be collected at all sites
and in their entirety;
Benthic samples should always be collected. Any sediment size is acceptable so long
as the definition of a "successful grab" is met (see Section 6.1.3);
Sediment composite material of sand-sized sediment grain or smaller, should be
collected;
o Since there may be cases where only a limited amount of sediment can be
acquired for the sediment chemistry, characterization, and toxicity composite, the
listing given below provides the expected sample in order of preference:
1) Organics/Metals
2) Total Organic Carbon (TOC)
3) Silt/Clay (Grain size)
4) Toxicity
o Flag and note the reason for limited sediment sample collections;
Fish collection for ecological contaminant analysis. For the ecological assessment, fish
collection may be conducted anywhere within a 500 m radius of the X-Sites. Successful
deployment of fish collection gear or the absence of fish in the catch should not
necessarily be used as a determining factor for rendering a site "unsampleable". Human
health fish sampling (subset of Great Lakes sites) requirement is covered separately.
4.1.6 Secondary Sediment Collection Areas
All water, benthos and sediment samples are expected to be collected at the same location,
as close to the X-Site as possible. However, there may be circumstances that arise that require
the field crew to relocate in order to successfully complete sampling at a site; specifically for
sediment samples. If benthos and/or sediment are collected from a secondary location, in situ
measurements and water collections do not need to be resampled. For these situations, a
guideline for locating a secondary sediment sample collection area follows:
If an acceptable sediment grab can not be obtained at the X-site, it is permissible to
move around within the 37 meter margin (of the X-site) to obtain the sediment sample,
using the site relocation method described previously (this is still considered the primary
sediment sample collection area). Mark the circle on the Sample Collection Form
indicating that sediment was collected within 37 meters of the X-site. Acceptable
means:
1) A sediment grab that meets the criteria for benthic samples; or
2) Enough sediment can be collected that will allow the crew to collect the
sediment surface sub-sample required for the sediment composite that
will be used to send to send to the laboratory for abiotic indicator analysis
(e.g., organics/metals, TOC, grain size, toxicity).
In cases where sediment sampling can be successfully conducted in a secondary
sediment collection area (e.g., > 37 m radius but within a 100 m radius (-0.05 nm) of the
X-site), then the field team may do so without having to re-collect the water samples.
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page 36
Mark the circle on the Sample Collection Form indicating that sediment was collected
between 37 and 100 meters from the X-site. Indicate in the comments section
approximately how far from the X-site and in what direction the sediment was collected.
Indicate the relative location of the sediment collection on the map on the back of the
Site Verification Form. The data will be flagged for subsequent review.
In Great Lakes sites only, teams may move out to a maximum distance of 500 meters
from the X-site in repeated attempts to locate suitable sediment sampling locations (after
attempting to collect sediment from within the primary and secondary locations). Mark
the circle on the Sample Collection Form indicating that sediment was collected between
100 and 500 meters from the X-site. Indicate in the comments section approximately
how far and in what direction the sediment was collected. Indicate the relative location
of the sediment collection on the map on the back of the Site Verification Form. The
data will be flagged for subsequent review.
If a suitable location to collect sediment samples has not been found after a minimum of
3 collection attempts inside each of the acceptable relocation areas, then sampling is
considered "complete" for the site. All appropriate field form flags and explanations
should be filled in. NOTE: More sediment grab attempts may be completed at the
discretion of the field team leader.
4.1.7 Habitat Assessment
Indicate on the site verification form the basic habitat type and bottom composition present
at the X-site. Note the presence and type of any marine debris, submerged aquatic vegetation
(SAV), and/or macroalgae present in the area.
4.1.8 Site Photograph
Taking site photographs is an optional activity that is encouraged, but should be considered
if the site has unusual natural or man-made features associated with it. If you do take
photographs with a digital camera at a site, date-stamp the photograph and include the site ID.
Alternatively, start the sequence with one photograph of an 8.5 x 11 inch piece of paper with the
site ID, waterbody name, and date printed in large, thick letters. After the photo of the site ID
information, take any additional photos you find interesting after this first picture. Keep a log of
your photographs and briefly describe each one. EPA encourages crews to submit digital
pictures to the regional and headquarters contacts for use in NCCA assessment materials.
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page 37
NCCA2010 SITE VERIFICATION (Front)
SITE NAME: G(JLF Of MEXICO
SITE ID: NCCA10 LAOOOO
DATE: Od lO I . /. 2 . ฐ . 1 . ฐ . VISIT: * 1 ฐ 2
STSrreฐF L A STATION DEPTH(m): ฃ> () TEAM: LA t
DID YOU SAMPLE THIS SITE?
0 YES |f YES. check one below
SAMPLEABLE (Choose method used)
Marine
O Great Lakes
ARRIVAL TIME: Q J : l{ &
DEPART TIME: ) ~$ ' , 3|Q[
Site verified by (fill in all that apply): GPS
O Other (Describe Here):
Coordinates Latitude North
TARGET Decimal Degrees 2 t '722
ACTUAL Decimal Degrees ^. ^ - 722
O NO If NO. check one below
NON-SAMPLEABLE-PERMANENT-ReplaceSite
O Map Error
O Site too shallow for navigation/sampling
O Unsafe ^%^
NON-SAMPLEABLE-TEMPORAr%ฃ-Rj}schedule
O No Access rf, *%. J*
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O Other (Explain in commenUfsOC,/1
VERIFICATION INFORMATION $ ^ "^
O Local Contact O Signs O Rd^s ^ O Topo. Map
QfiJWJ/irified (Explain in Comments)
LOCATION A "\^^
Longltur^yst Satellites X-SITE WITHIN 37M?
A , ^i^*%y *YES ฐNฐ
/I /x /iv A | <)fe^7lo t\ r~ "^ .-. -.
ID (J C./T 1 4 ,/.jT> O L),^-. O<3
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7O 0,^1,5,2,8,6.^,0. .WGSS4 ,
HABITAT TYPE: O Tidal River O Open Water O MailhAMind Embayment O Inter-Tidal O Rivermouth
O'^tKor, explain:
BOTTOM TYPE: O Coral Reef O Oyster Be
c
Debris Present?: \ If Yes, TYPE: %^
YES O NO ' O Glass O Piastil^tj^
J*COGrtssBed O Sand O Rocky/Shell O Hardpan Mud
\ OOther, explain:
;^ PiA/v)T,$
ood OCans Other, exolain: RAPT ซฃ TiCftiR AA)0 FtOATlAJCV
SAV Present?: O Yes^ป t$& ABUNDANCE: (Sparse, dense, etc)
Macroalgae Present?: %%"\> No ABUNDANCE: S?A(ฃ.Sฃ (Sparse, dense, etc)
GENERAL COMME%^ C, ,Tฃr ,ฃ LOCATE.t> 2.6, NAOTICAC MlC^S OFF Of
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03^31/2010 NCCA Site Verification
8194026369
Figure 4-3. Example Site Verification Form (Front)
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page 38
NCCA2010 SITE VERIFICATION (Back)
Ftevfewvdby
SITE NAME:
QF
DATE: QV fQ I / 2
VISIT: 1 ฐ 2
SITEID;
NCCA10
TEAM:
SKETCH MAP -Arrow Indicates North; Mar* site L=Launcti X=lndex F = Fishing Area
NOTE: If an outline map Is attached here, use a continuous strip of clear tap* across tha lop edge.
You can also attach a separate sheet with the outline map on It
t
\
O
"V^"
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PERSONNEL
NAME
Bio/Chem
Sampling
Fish
o
o
o
o
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O
O
O
O
03/31/2010 NCCA Site Verification
Figure 4-4. Example Site Verification Form (Back)
1975026369
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page 39
Table 4-2. Site Verification Procedures
1. Create a waypoint in the GPS unit that corresponds to the target X-site coordinates provided by EPA
in the site list. This can be done ahead of time in the office.
2. Record the coordinates of the target X-site on the Field Verification Form in decimal degrees (Target
field).
3. Navigate to the target X-site while noting the distance (in meters) from the given coordinates.
4. Navigate the sampling vessel as close as possible to the target X-site (you must be no more than 0.02
nm or 37 meters from the target X-site).
5. Anchor the sampling vessel in such a way as to minimize the possibility of the anchor(s) dragging or
becoming dislodged.
6. Record the time of arrival at the X-site.
7. Record the coordinates of the actual X-site on the Field Verification Form in decimal degrees (Actual
field).
8. Create a new GPS waypoint shortly after anchoring and monitor the GPS throughout the sampling to
ensure that the sampling vessel has not drifted away from the X-site due to anchor drag.
9. Indicate any and all methods that were used to verify that you are at the correct location.
10. Measure and record the water depth at the X-site on the form.
11. Determine if the site is sampleable - See Site Evaluation Guidelines.
12. If the site is non-sampleable or inaccessible and cannot be relocated within the designated area,
indicate the reason on the form. No further sampling activities are conducted. Replace the site with
the first oversample site on the estuary/state list. Notify the EPA Regional Coordinator and Field
Logistics Coordinator that the site was replaced and submit the verification form to the Information
Management Coordinator.
13. If the site is sampleable, record the sampling method being used (marine or Great Lakes).
14. Record the general habitat type and the dominant bottom type present at the sampling site. In many
sites, it may not be possible to record the bottom type until after the sediment collections are
performed.
15. Record the presence and type any debris or submerged aquatic vegetation (SAV) present.
16. Make any general comments about the site that may be important during the data review portion of
the assessment or any unusual characteristics about the site.
17. Record directions to the launch site from an easily recognizable location (city or major road
intersection).
18. On the back side of the Field Verification Form, draw a simple sketch of the area. Include the relative
locations of the shoreline, launch point, X-site, sediment and fish collection location. Include any other
specific attributes of the site that may be important during the data processing portion of the
assessment. A printed or copied section of a map with the pertinent information may be submitted in
place of the scene sketch.
19 Record the name of crew member and indicate their nrimarv duties
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page 40
5.0WATER QUALITY MEASUREMENTS
5.1 Water Quality
This section describes the procedures and methods for the field collection and analysis of
the water quality indicators (in situ measurements, water chemistry, Secchi disk transparency,
and light attenuation) from freshwater and marine coastal areas.
5.1.1 In Situ Measurements of Dissolved Oxygen, pH, Temperature, Salinity,
Conductivity, Transparency, and Light Attenuation
5.1.1.1 Summary of Method
Measure dissolved oxygen (DO), pH, temperature, and salinity (marine sites) or conductivity
(freshwater sites) using a calibrated multi-parameter water quality meter (or sonde). Measure
water column transparency using a Secchi disk and light attenuation using a Photosynthetically
Active Radiation (PAR) meter. Take all the measurements at the X-site at the following depths:
0.1 m below the surface, 0.5 meters below the surface, every 1 meter from depths of 1.0 to 10.0
meters, and every 5 meters thereafter if the site is greater than 10m. Take the last set of
measurements at 0.5 m from the bottom. Be sure the site depth is accurately measured and
recorded before taking the water quality measurements. Take care to avoid the probes
contacting bottom sediments, as the instruments are delicate. Refer to table 5-3 for detailed
instructions on taking the hydrographic profile.
The hydrographic profile will include a full set of measurements on both the downcast
(lowering the probe through the water column), and the upcast (as the probe is brought back to
the surface). The downcast and upcast measurements will be taken at the same depths.
5.1.1.2 Equipment and Supplies
Table 5-1 provides the equipment and supplies needed to measure transparency, light
attenuation, dissolved oxygen, pH, temperature, and salinity/conductivity. Record the
measurements on the Field Measurement Form, as seen in Figures 5-1 and 5-2.
Table 5-1. Equipment and SuppliesDO, pH, Temperature, Salinity/Conductivity, Transparency,
and Light Attenuation
For taking measurements and
calibrating the water quality meter
For recording measurements
Multi-parameter water quality meter with pH, DO
temperature, and salinity/conductivity probes.
Extra batteries
De-ionized water (lab certified preferred, but not
Calibration cups and standards
QCS calibration standard
Barometer to use for calibration
Thermometer
Secchi disk
PAR meter with independent datalogger
required)
Field Measurement Form (see Figures 5-1 and 5-2)
Pencils (for data forms)
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page 41
NCCA2010 FIELD MEASUREMENT (Front)
Revlowad by (Initial):
W W
SITEID: NCCA10LAOOOO "^ Ak, 1.0, | , /, 2 0 1 ^
CALIBRATION INFORMATION
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Instrument ID number: \Ol^2.| Operator: ^J, 5A^T"oM
TEMPEFiATURE
DO
pH
CONDUCTIVITY
Thermometer Sensor Reading
Reading (ฐC) ('C(
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Flag Comments
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Cal. STD 1 Description Cal. STD 1 Value Cal. STD 2 Description '\'" Cal. STD 2 Value Flag
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QUALITY CONTROL CHECK (Perform at least once per week)
TIME:
l_
QC BATCH #:
Date Prepared:
COMMENTS:
17.:.0,Q.
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04/01/2010 NCCA Raid Measurement
9117512028
Figure 5-1. Example Field Measurement Form (Front).
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page 42
y NCCA 2010 FIELD MEASUREMENT (Back) R.vi.w.dbjMkiii!
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Figure 5-2. Example Field Measurement Form (Back).
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page 43
5.1.1.3Secchi Disk
The Secchi disk is used to give a measurement of the transparency of the water column,
also called the Secchi depth. This measurement is made at every station and is recorded on the
datasheet. A 20 cm black and white Secchi disk is held by a non-stretch line that is marked in
two tenths of a meter intervals.
Table 5-2 presents step-by-step procedures for measuring water column transparency. If
the range of measurements for the three sets of depth readings is greater than 0.5 m, the entire
process should be performed again. No sunglasses or any other devices should be used to
shade the eyes while this procedure is being performed. The Secchi depth should be
determined from the shady side of the boat during daylight hours.
Table 5-2. Sampling ProcedureSecchi Disk.
1. Remove sunglasses, hats or other devices used to shade the eyes.
2. Slowly lower the Secchi disk on the shady side of the boat until it is no longer visible and note the
depth using the markings on the line (interpolate between markings to the nearest 0.1 meter).
If the disk hits the bottom, meaning the Secchi depth is greater than the water depth, note this on the
datasheet by marking the "Yes" circle under "Clear to Bottom?" and recording the depth of the water
in both the "disappears" and "reappears" boxes.
3. Slowly raise the Secchi disk until it just becomes visible and note the depth.
4. Perform steps 1 and 2 two more times, noting both disappearance and reappearance depths each
time.
5. Record all six measurements on the Field Measurement Form.
6. Flag any measurements that the team feels needs further comment or when a measurement cannot
be made.
7. Repeat the entire process if the three sets of measurements vary by more than 0.5 m.
5.1.1.4 Multi-Probe Sonde
Dissolved Oxygen Meter
Calibrate the DO meter prior to each sampling event and record the calibration values on
the Field Measurement Form. It is recommended that the probe be calibrated in the field against
an atmospheric standard (ambient air saturated with water) prior to launching the boat. In
addition, manufacturers typically recommend periodic comparisons with a DO chemical analysis
procedure (e.g., Winkler titration) to check accuracy and linearity.
pH Meter
Calibrate the pH meter prior to each sampling event and record the calibration values on the
field measurement form. Calibrate the meter in accordance with the manufacturer's instructions
and with the team agency's existing Standard Operating Procedure (SOP). You must also
conduct a quality control check with the provided standard to verify the calibration and
periodically evaluate instrument precision (see Section 3.1.2). Once a week, each crew must
check their multi-probe against the QCS provided in each site kit. Any irregularities must be
reported to either the Site Kit Coordinator or the Field Logistics Coordinator immediately, and a
new QCS requested. QCS values are also recorded on the Field Measurement Form.
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Field Operations Manual Date: April 23, 2010
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After all in situ measurements have been completed for the sampling day, the team must
perform a post-measurement calibration check of the pH meter to detect any drift from the
values. To do this, measure the pH of the calibration standard that was used earlier in the day
to calibrate the instrument. Record these values on the Field Measurement Form. If significant
drift is detected, it may indicate that the meter is in need of service.
Temperature Meter
Check the accuracy of the sensor against a thermometer that is traceable to the National
Institute of Standards (NIST) at least once per sampling season. The entire temperature range
encountered in the NCCA should be incorporated in the testing procedure and a record of test
results kept on file.
Salinity/Conductivity Meter
Calibrate the salinity/conductivity meter prior to each sampling event and record the
calibration values on the field measurement form. Calibrate the meter in accordance with the
manufacturer's instructions. The entire salinity/conductivity range encountered in the NCCA
should be incorporated in the testing procedure and a record of test results kept on file. You
must also conduct a quality control check with the provided standard to verify the calibration and
periodically evaluate instrument precision (see Section 3.1.2). Once a week, each crew must
check their multi-probe against the QCS that was supplied in each base kit. Any irregularities
must be reported to the Field logistics coordinator immediately. QCS values are also recorded
on the field measurement form.
After all in situ measurements have been completed for the sampling day, the team must
perform a post-measurement calibration check of the conductivity meter to detect any drift from
the values. To do this, measure the conductivity of the calibration standard that was used
earlier in the day to calibrate the instrument. Record these values on the Field Measurement
Form. If significant drift is detected, it may indicate that the meter is in need of service.
Table 5-3 presents step-by-step procedures for measuring dissolved oxygen, pH,
temperature, and salinity (marine sites) or conductivity (freshwater sites).
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page 45
Table 5-3. Sampling ProcedureTemperature, pH, Dissolved Oxygen and Salinity/Conductivity
1. Check meter and probes and calibrate according to manufacturer's specifications and record the
calibration values on the field measurement form.
2. Check the calibration against the provided QCS solution for pH and salinity/conductivity and record
the results on the field form as the QCS Measured value. This should be done at least once a
week.
3. Record the true value of the QCS solution from the stock solution container on the field form as
QCS True.
4. Measurements are taken at the X site at multiple depths. Measurements of all four parameters will
be recorded at each depth.
5. Measure the total water depth to the nearest 0.1 meters and record on the hydrographic profile
form.
6. Lower the sonde in the water and measure DO, pH, temperature, and salinity/conductivity at the
following depths: 0.1 m below the surface, 0.5 m below the surface, every 1 meter from depths of
1.0 to 10.0 meters, and every 5 meters thereafter if the site is greater than 10 m. Take the last set
of measurements at 0.5 m from the bottom.
7. Repeat the full sets of measurements at each of the same depth intervals as the probe is retrieved.
8. The first set of measurements will be placed in the "downcast" section of the data sheet. Take
measurements at the same depth intervals on the return cast to the surface and record in the
"upcast" section. Two examples are provided below that illustrate the depths at which
measurements will be taken.
EXAMPLE 1: EXAMPLE 2:
Water Depth = 7.2 meters Water Depth = 23.9 meters
0.1 m 0.1 m
0.5 m 0.5 m
1.0m 1.0m
2.0 m 2.0 m
3.0 m 3.0 m
4.0 m 4.0 m
5.0 m 5.0 m
6.0 m 6.0 m
6.7 m 7.0 m
8.0 m
9.0 m
10.0m
15.0m
20.0m
23.4m
9. Record the measurements on the Field Measurement Form.
10. Flag any measurements that the team feels needs further comment or when a measurement
cannot be made.
11. After all in situ measurements have been completed for the sampling day, perform a post-
measurement calibration check of the pH and conductivity probes. Record these values on the
Field Measurement Form.
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5.1.1.5 Photosynthetically Active Radiation (PAR) Meter
A PAR meter, attached to a data logger such as a LI-CORฎ, is used to obtain a vertical
profile of light in order to calculate the light attenuation coefficient at each station. PAR sensors
require no field calibration, however, they should be returned to the manufacturer at least every
2 years for calibration. PAR measurements are taken at the same depths as other water column
indicators. Table 5-4 presents step-by-step procedures for measuring light attenuation.
Table 5-4. Sampling ProcedureLight Attenuation (LI-1400 Datalogger).
1. Connect a deck sensor and an underwater sensor to the PAR meter. Make sure the correct
calibration factors are entered for each probe. These are supplied by the manufacturer and are
specific to each individual probe.
2. Place the deck sensor on the boat in a location where it is not shaded.
3. Turn on the LI-1400 meter.
4. Press the View key.
5. Using the left or right keys navigate to "NEW DATA" and press Enter.
6. Using the left or right keys navigate until channel 111 is displayed; this shows the instantaneous
reading for that channel. Scrolling down will allow viewing of 2 channels at once.
7. Lower the underwater sensor on the SUNNY (or at least unshaded) side of the boat to a depth of 10
cm (represents "surface").
8. When all sensors are in place at the desired depths, it is important to record both readings at the
same instant to ensure there is no change in light availability. One option is to use the datalogger by
pressing ENTER and manually storing the instantaneous readings from all attached sensors.
9. To review the saved data, press Esc then use the right or left key to select "LOG DATA" press Enter.
10. Select "View=ALL", press Enter.
11. Use the down key to scroll through stored data by date and time to find the data that was just logged;
press Enter to access logged data. Use the down key to view both of the sensor readings.
12. Record the values from both sensors (/jE/m2/s), along with the water depth of the underwater sensor,
on the datasheet. Record the deck sensor reading in the ambient (AMB) column, and the underwater
sensor reading in the underwater (UW) column.
13. Lower the underwater sensor to 1.0 meter, repeat steps 8 through 11 to capture the values, and
record the values from both sensors, along with the depth of the underwater probe.
14. Repeat measurements at the following schedule (same as other water quality measurements):
0.5 meters
Every 1 meter from 1.0 m to 10.0 m
Every 5 meters thereafter for sites greater than 10 meters
0.5 meters from the bottom
15. If the bottom is impacted with the meter, allow 2-3 minutes for the disturbed conditions to settle
before taking the reading.
16. If the light measurements become negative before reaching the bottom measurement, terminate the
profile at that depth.
17. Repeat the process on the upcast and record values on the datasheet.
Note: Pressing the On/Off key will only turn off the screen. To shutdown the LI-1400 press the Fct key
and use the right or left keys to navigate to "SHUTDOWN". Press Enter to shutdown.
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5.2 Fecal Indicator (Enteroccoci)
The collection time of the Enterococci sample may vary based on whether the team will be
collecting fish for fish tissue samples and whether those collections will be performed using an
active or passive fishing method. Refer to section 2.1 and Figures 2-1, 2-2, and 2-3 for more
information. In short, if the team is not fishing, or is using a passive fishing method, the
Enterococci collection should take place immediately following the hydrographic profile. If the
team is using active fishing methods, the collection of the Enterococci sample should take place
at the end of the sampling day. This is based on the need to protect the Enterococci sample
from potential contamination and to minimize holding times once the sample is collected. There
is a strict 6 hour window from the time of collection of the Enterococci sample to the time when
four aliquots of sample are filtered and all four filters frozen.
5.2.1 Summary of Method
Collect a fecal indicator sample at the X-site. Use a pre-sterilized, 250 ml_ bottle and collect
the sample at about 0.5 meters below the water surface. For smaller vessels, this can be
accomplished with a gloved hand. For larger vessels, the bottle may need to be affixed to a pole
dipper. Following collection, add a sodium thiosulfate tablet, shake well, place the sample in a
cooler, chill for at least 15 minutes, and maintain on ice prior to filtration of four 50 ml_ volumes.
(Samples must be filtered and frozen on dry ice within 6 hours of collection). In addition to
collecting the sample, look for signs of disturbance throughout the reach that would contribute to
the presence of fecal contamination to the waterbody. Record these disturbances on the Site
Assessment Form (Figure 8-2).
5.2.2 Equipment and Supplies
Table 5-5 provides the equipment and supplies needed to collect the fecal indicator sample.
Record the sample data on the Sample Collection Form (Figure 5-4).
Table 5-5. Equipment and Supplies List for Fecal Indicator Sampling
For collecting samples
nitrile gloves
pre-sterilized, 250 ml sample bottle
sodium thiosulfate tablet
Wet ice
cooler
For recording
measurements
Sample Collection Form
Fecal Indicator sample labels (4 vial labels and 1 bag label)
Pencils (for data forms)
Fine tipped indelible markers (for labels)
Clear tape strips
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5.2.3 Sampling Procedure
The procedure for collecting the fecal indicator sample is presented in Table 5-6.
Table 5-6. Procedure for Fecal Indicator (Enterococci) Sample Collection
1. Put on nitrile gloves.
2. Collect the sample over the side of the boat with a gloved hand or pole dipper (on larger vessels).
3. Lower the un-capped, inverted 250 ml sample bottle to a depth of 0.5 meters below the water
surface, avoiding surface scum, vegetation, and substrates. Point the mouth of the container away
from the boat. Right the bottle and raise it through the water column, allowing bottle to fill
completely.
4. After removing the container from the water, discard a small portion of the sample to allow for
proper mixing before analyses.
5. Add the sodium thiosulfate tablet, cap, and shake bottle 25 times.
6. Store the sample in a cooler on wet ice to chill (not freeze). Chill for at least 15 minutes and do not
hold samples longer than 6 hours before filtration and freezing.
5.3 Water Chemistry Sample Collection and Preservation
5.3.1 Summary of Method
The water chemistry samples will be analyzed for chlorophyll-a, dissolved ammonia, nitrites,
nitrates, and phosphorus. Collect the water samples with either a pumped system or a water
sampling bottle such as a Niskin, Van Dorn, or Kemmerer bottle and transferred to a rinsed 250
ml_ amber Nalgene bottle. Water for the chlorophyll-a sample will be collected and transferred to
a separate 2 L amber Nalgene bottle. Store all samples in darkness on ice in a closed cooler.
After you filter the chlorophyll-a samples, the filters must be kept frozen until ready to ship. A
portion of the filtrate from the chlorophyll-a processing will be collected for the dissolved nutrient
sample. Note that the fecal indicator sample IS NOT collected with these samples.
Collect the samples at the X-site, 0.5 meters below the surface.
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5.3.2 Equipment and Supplies
Table 5-7 provides the equipment and supplies needed to collect water samples at the X-
site.
Table 5-7. Equipment and SuppliesWater Chemistry and Chlorophyll-a Sample Collection
For collecting samples
Water sampling device or water pumping system
Nitrile gloves
one 250 ml amber Nalgene bottle
one 2 L amber Nalgene bottle (chlorophyll-a)
Cooler with wet ice
Field Operations Manual and/or laminated Quick Reference Guide
For recording
measurements
Sample Collection Form
Field Measurement Form
Pencils (for data forms)
Fine-tipped indelible markers (for labels)
Clear tape strips
5.3.3 Sampling Procedure
Table 5-8 describes the sampling procedures for collecting water chemistry samples.
Table 5-8. Sampling Procedure for Water Chemistry and Chlorophyll-a Sample Collection
1. Collect the water chemistry samples at the X-site (located via GPS).
2. Put on nitrile gloves. Make sure not to apply sunscreen or other chemical contaminants until after
the sample is collected.
3. Using either a pumped system or a water sampling bottle, collect a water sample at 0.5 m below
the surface.
4. Rinse the pumped system or sampling bottle as well as the sample containers three times with
water from the site. Fill the 250 ml amber Nalgene bottle (for water chemistry) and the 2 L
amber Nalgene bottle (for chlorophyll-a) with sample water, and place in a cooler on ice. Make
sure the water chemistry label is complete and taped over and place samples in a cooler on ice at
4ฐC.
5. Record the collection data on the Sample Collection Form. Note anything that could influence
sample chemistry (heavy rain, potential contaminants) in the Comments section. If the samples
were not taken at the X-site, enter the GPS coordinates of the sampling location and the reason
for relocation in the comments field on the Sample Collection Form (Figure 5-4).
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Page 50
5.4 Phytoplankton
5.4.1 Summary of Method
In all Great Lakes sites, teams will collect a sample for Phytoplankton analysis. Collect this
sample from the X-site at the same time and depth as the other water samples. Fill a 1 liter
amber nalgene bottle with from the water sampler or pumped system. The phytoplankton
sample must be preserved with 10 mL of Lugol's solution within 2 hours of collection. Store the
samples in darkness inside a cooler with ice or in a refrigerator.
5.4.2 Equipment and Supplies
Table 5-9 provides the equipment and supplies needed to collect the phytoplankton sample
at the X-site.
Table 5-9. Equipment and SuppliesPhytoplankton
For collecting and
preserving samples
Water sampling device or water pumping system
Nitrile gloves
one 1L amber Nalgene bottle
Cooler with wet ice
Field Operations Manual and/or laminated Quick Reference Guide
Lugol's solution
For recording
Sample Collection Form
measurements . pencils (for data forms)
Fine-tipped indelible markers (for labels)
Clear tape strips
5.4.3 Sampling Procedure
Table 5-10 describes the sampling and preservation procedures for phytoplankton samples.
Table 5-10. Sampling and Preservation Procedure for Phytoplankton
1. Collect the water chemistry samples at the X-site along with the other water samples.
2. Put on nitrile gloves. Make sure not to apply sunscreen or other chemical contaminants until after
the sample is collected.
3. Using either a pumped system or a water sampling bottle, collect a water sample at 0.5 m below
the surface.
4. Fill the 1 L amber Nalgene bottle with sample water, and place in a cooler on ice. Make sure the
phytoplankton label is complete and taped over and place samples in a cooler on ice at 4ฐC.
5. The sample must be preserved by adding 10 mL of Lugol's solution to the bottle within 2 hours of
collection. Rotate the bottle gently to mix the sample.
6. Record the collection data on the Sample Collection Form. Include the depth of collection, time of
collection, and time of preservation.
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Page 51
5.5 Underwater Video
At all Great Lakes sites, a 1 minute video image of the substrate will be collected using an
underwater video camera system. The video will be enhanced and examined in the lab to
visually document the bottom composition, and record the presence or absence of zebra
mussels, Cladophora, or other organisms.
5.5.1 Summary of Method
High quality underwater video will be best achieved if the field crew deploys the camera and
records the video at approximately the same time as the in situ measurements and water
collection activities. Avoid heavy disturbance of the bottom with anchors or sediment samplers
before capturing the video images.
While anchored at the X-site, lower the camera into the water on the windward side of the
boat. One person is needed to operate the DVR and one to lower the camera. The person
operating the DVR should instruct the camera person on descent speed and depth of camera.
When a clear view of the bottom can be seen, start recording the video by pressing the record
button. Continue recording until you have captured 1 min of good bottom footage. In low light
conditions, turn on the camera light by pressing the red button on the DVR end of camera cable.
Experiment with the light while monitoring the screen for best picture results.
5.5.2 Equipment and Supplies
Table 5-11 provides the equipment and supplies needed to record the underwater video at
the X-site.
Table 5-11. Equipment and SuppliesUnderwater Video
For recording
underwater video
Seaviewer underwater camera
Seaviewer digital video recorder (DVR)
Seaviewer SeaTrak GPS overlay
Garmin Etrex GPS
Camera cable (100')
Cable from GPS overlay to DVR
Cable from GPS overlay to GPS
12v18ah battery
Charger for 12v battery
Power cord (DVR .Camera ,GPS overlay)
Power adapters (110VAC - 12VDC) (3) for camera, DVR, and GPS overlay
18gbSD card
Stop watch (or similar time keeping device)
Seaviewer case (all components will fit into case for transport)
10 amp fuses (Automotive blade (large) type)
AA batteries (for GPS)
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5.5.3 Initial Setup of Underwater Camera System
Underwater camera systems will be assembled and set up prior to shipment to field crews.
However, information contained within this section will allow a field crew to verify equipment
setup or troubleshoot potential connection problems. The underwater camera system and
cables should be set up as shown in Figure 5-3. The system should not be disassembled
between sites other than to remove the battery clips. Initial one-time setup of the camera
system GPS unit is described in Table 5-12.
camera
gps
etrex
cable
- gps Receiver
liver *
gps|ovErlay
IฐT. "
. VidGO J '
out
sd card slct / ush
light switch
power to DVR
. power cord.
Figure 5-3. Setup Diagram of Underwater Video System
Table 5-12. Initial Setup of Camera System GPS
Set the GPS to output NMEA data in the GPS Menu section of the settings to send position
information to the GPS overlay system. (This step will be completed prior to shipment of the system,
but the steps below can be completed to verify correct setup).
1. Press "page" button 4 times to reach menu page.
2. Select "set up" by pressing arrow down button until "set up" is highlighted, then press enter.
3. Select "interface" by pressing arrow down button until "interface" is highlighted, then press enter.
4. Press enter again, select "NMEA out" by pressing arrow down button until "NMEA out" is
highlighted, then press enter.
5. Press page button 3 times to return to satellite tracking page.
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5.5.4 Underwater Video Recording Procedure
Table 5-13 describes the procedure for recording the underwater video at the X-site. Table
5-14 describes the procedure for archiving the video file after the recording has been
completed.
Table 5-13. Procedure for Recording Underwater Video
1. Power up the GPS and wait until it displays: "ready to navigate" before proceeding.
2. If the GPS is not set to output NMEA data, see Table 5-12
3. Send power to the camera, GPS overlay and DVR by attaching alligator clips to the 12v battery.
Attach red clip to the positive (+) terminal and black clip to the negative (-) terminal.
4. Turn on the GPS overlay by pressing its power button. The green light will illuminate.
5. Turn on the DVR by pressing the power button (upper right side of DVR) for 3 seconds. A flash
screen will appear for a short time then disappear. NOTE: DO NOT PRESS POWER ON AGAIN
DURING THIS TIME! A windows type menu screen will appear.
6. Initialize the DVR by pressing the video button located at top right of the DVR unit (not on the
screen). A video image from the camera should appear on the DVR screen with a latitude /
longitude display. (If not, see the trouble shooting section supplied with manufacturer's literature).
7. Lower camera into the water on the windward side of the boat. One person is needed to operate
the DVR and one to lower the camera. The person operating the DVR should instruct the camera
person on descent speed and depth of camera.
8. When a clear image of the bottom is displayed, hold the camera as still as possible and start
recording by pressing the record button (located at top right of the unit, to the right of the video
button). The word "Recording" appears on the screen in red for 10 sec, then disappears. (To
pause recording, press the enter button then press again to resume recording.)
9. Continue recording until you have captured 1 minute of good bottom footage.
10. In low light conditions, turn on the camera light by pressing the red button on the DVR end of
camera cable. Experiment with the light while monitoring the screen for best picture results.
11. Stop recording by pressing the video key (top of unit), or the X button.
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Field Operations Manual Date: April 23, 2010
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Table 5-14. Procedure for Archiving Underwater Video Files
Upon completing the 1 minute of underwater video, it is important to verify that the video has been
saved, record the file name on the Sample Collection Form, and preview the video to ensure
adequate quality.
1. Select browser by pressing the enter button (upper right key on front of DVR).
2. Arrow down to "DVR".
3. Select "DVR" by pressing the enter button (upper right key front of DVR).
4. Arrow down to the last file listed. This should be the video you just recorded.
5. Record the file name on the Sample Collection Form. The format of the file is:
DVRyymmdd_hhmm_xxx.avi (yymmdd is the date in year, month and day; hhmm is the time in
hours and minutes; xxx is a file number assigned by the DVR, typically 001; and avi is the file
format). Check that the date and time on the file name match the date and time of the recording
you just made.
6. Press enter to play video to evaluate the quality of the video.
7. If the video clearly shows the composition of the bottom then the video is deemed acceptable;
continue to step 9.
8. If the video is unviewable or is of poor quality, repeat the recording steps in Table 5-13.
9. Shut down the system by the following the steps below.
a. Power down the DVR by pressing and holding the power button (upper right side).
b. Power down the GPS overlay by pressing the power button.
c. Power down the camera by disconnecting the alligator clips from the battery posts.
d. Power down GPS by pressing and holding its power button.
10. Recharge the 12v battery at the end of each day.(It is a good idea to assign this task to an
individual crew member.)
11. Back-up files to the SD card by following the steps below (do this as soon as possible to back up
your data).
a. Insert SD card into the SD slot (top left on DVR).
b. Power on the DVR.
c. Arrow over to "Browser" (picture of monitor with magnifying glass).
d. Select "Browser" by pressing the enter button (upper right key on front of DVR).
e. Arrow down to "DVR".
f. Select "DVR" by pressing the enter button (upper right key front of DVR).
g. Arrow down to the file you want to copy to the SD card.
h. Press the "Tools" button (lower left key).
h. The "CCP" option will be highlighted. Press the enter button.
i. The "copy" option will be highlighted. Press the enter button.
j. A second path will appear listing the SD card as an option. Arrow down to SD card.
k. Press the enter button (upper right key front of DVR)
I. Press the "Tools" button (lower left key).
m. "Paste" will be highlighted. Press enter.
NOTE: backing up files to your computer is also suggested; these files are/can be large so this may
not be an option for you. You can either insert the SD card directly into the computer to copy, or use
the supplied USB cable to plug into your computer. Your computer will see the DVR hard drive as
another drive and you can copy and paste them to a file on your computer.
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Page 55
m NCCA 2010 SAMPLE COLLECTION FORM - (Front)
Reviewed by Jv-*
SITEID: NCCA10 |OCfl DATE: Q fe /O i / 2 ฐ 1 ฐ
WATER CHEMISTRY . CHLOROPHYLL and NUTRIENT COLLECTION (0,5m)
Water Chemistry
(Non-Filtered)
999. I.O.I.5
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339.1.02.
Nutrients
(Filtered)
999.1.0.3.
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Frozen
Chilled
*
Comments
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Voi Filtered : ; .
(ml) Comments
1000
Comments
No Sairป,5e*3onected Q
V
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^ , %
Use comment section to explain: No measurement, suspect measurement or observation made. < ,
j-V *i
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ENTEROCOCCI (Target Volume
Sample ID
.99 9. 8 .6.ft
Filter Blank
999.BJ&9
F
Tirno
Collided
IM45
Depth
Collected
(m)
Q,S
Sample
Volume
(mL|
250
Flit. Start
Time
(hhmm)
\loOQ
."?" f.- ^
= 250 m
*
Voluma '
Fill 0 Vป2??
|S/^| ISZf\
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Volume
, . (Target'
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FHL2
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i '' No Sample Collected O
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IFUL 3
50
Flit 4
50
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FlltS
20
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20
Vol.
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Rinse
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Fill End
Time
(hhmm)
1730
Time
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(hhmm)
IftOO
Flag
-j^.
Flag codes: K - No m.Murปin.nt mad., U = Suspect measurement? F1.F2, Me. - flags m\tan> by each field crew. Explain all flags In comments.
Flag
'Comments
GREAT LAKES ONLY
PHYTOPLANKTON(I-L)
No Sample Collected O!
Sam^lfft \
99-9"lt>0
; - '
Prtsorved
Depth
Collected
(m)
0,5
Time
Collected
(hhmm)
I045
Time
Preserved
(hhmm)
\ I*^O
Comments
Undar water video camera Digital Video Recording Nฐ SamP" Collected Q
Filename Transferred
Format: DVRyymmdd_hhmm_xxx.avi to 3D Card Comments
;DVfM.O.O.fe.O.I , I 030 .P.O. i. 'avl
8935052620
04/22/2010 NCCA Sample Collection
Figure 5-4. Example Sample Collection Form (Front)
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6.0SEDIMENT COLLECTIONS
6.1 Sediment Collections
Sediments are collected for a variety of analyses. One sample is collected for benthic
species composition and abundance, and additional sediment grabs are collected for chemical
analyses (organics/metals and TOC), grain size determination, and for use in acute whole
sediment toxicity tests. The number of grabs needed may vary based on the sediment
characteristics. While the biology grab is being processed (sieved), grabs should be collected
for chemistry, grain size and toxicity tests. These grabs will be composited, mixed and split into
four separate sample containers. A minimum of 4L of sediment will be required for the chemistry
and toxicity samples.
6.1.1 Summary of Method
A 1/25 (0.04) m2, stainless steel, Young-modified Van Veen Grab (or similar) sampler is
appropriate for collecting sediment samples for both biological and chemical analyses. The top
of the sampler is either hinged or otherwise removable so the top layer of sediment can be
easily removed for chemical and toxicity sample collection. This gear is relatively easy to
operate and requires little specialized training. For sampling in the Great Lakes, a standard
Ponar grab (box size 22.9 cm x 22.9 cm with depth of 9 cm) with removable top screens may be
more appropriate (USEPA 2001). Record the dimensions and sample area of the grab used on
the Sample Collection Form, side 2. The area of sediment the grab collects is important for data
analysis. If the grab sampler size is less than 0.03 m2, take two grabs for the benthic
macroinvertebrate collections and composite the sediment into the sieve.
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6.1.2 Equipment and Supplies
Table 6-1 provides the equipment and supplies needed to collect sediment samples at the
X-site. Record the Sediment Sample Collection and Preservation data on the Sample Collection
Form.
Table 6-1. Equipment and SuppliesSediment Collection
For collecting samples
Young-modified Van Veen (or
Ponar) grab with grab stand
Weights and pads for grab
Nitrile gloves
Tub or bucket
0.5 mm stainless steel sieve (1.0
mm for CA, OR, WA)
Sieve box or bucket
Electrical tape
Fine-tipped forceps
Wide-mouthed funnel
Alconox
Formalin
Rose Bengal Stain
Borax
Centimeter ruler
Squirt bottle
Stainless mixing pot or bowl with lid
Cooler with wet ice
Stainless steal or Teflon spoons
1 L Nalgene bottle(s) for benthos
1 gallon plastic bucket for toxicity
500 ml glass jar for organics and
metals
125 ml Nalgene jar for grain size
60 ml Nalgene jar for TOC
Field Operations Manual and/or
laminated Quick Reference Guide
For recording
measurements
Sample Collection Form
Field Measurement Form
Pencils (for data forms)
fine-tipped indelible markers (for labels)
Clear tape strips
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6.1.3 Sampling Procedure
Table 6-2 describes the sampling procedure to obtain sediment samples.
Table 6-2. Sampling Procedure for Sediment Collection
1. The sampler must be thoroughly washed with Alconox prior to use at a station, then rinsed with
ambient seawater/fresh or lake water to ensure no sediments remain from the previous station.
2. Attach the sampler to the end of the winch cable with a shackle and tighten the pin.
3. Cock the grab.
4. Lower the grab sampler through the water column such that travel through the last 5 meters is no
faster than about 1 m/sec. This minimizes the effects of bow wave disturbance to surficial
sediments.
5. Allow a moment for the sampler to settle into the substrate and then slack off on the cable. Letting
the cable go slack serves to release the jaws of the sampler so they will close as the sampler is
retrieved.
6. Retrieve the sampler and lower it into its cradle on-board. Open the top and determine whether
the sampling is successful or not. A successful grab is one having relatively level, intact sediment
over the entire area of the grab, and a sediment depth at the center of at least 7 centimeters for
the benthic macroinvertebrate grab (see Figure 6-1). Grabs containing no sediment, partially filled
grabs, or grabs with shelly substrates or grossly slumped surfaces are unacceptable. Grabs
completely filled to the top, where the sediment is in direct contact with the hinged top, are also
unacceptable. It may take several attempts using different amounts of weight to obtain the first
acceptable sample. The more weight added, the deeper the bite of the grab. In very soft mud,
pads may be needed to prevent the sampler from sinking in the mud. If pads are used, the rate of
descent near the bottom should be slowed even further to reduce the bow wave.
7. If, after several attempts, only grabs less than 7 centimeters deep can be obtained, use the next
successful grab regardless of the depth of sediment at the center of the grab. Flag the collection
on the data form and be sure to accurately record the depth of the grab.
8. Carefully drain overlying water from the grab. If the grab is used for benthic community analysis,
the water must be drained into the container that will receive the sediment to ensure no
organisms are lost.
9. Enter notes on the condition of the sample (smell, substrate, presence of organisms on the
surface, etc.) on the data sheet (Figure 6-2).
10. If the grab sampler size is less than 0.03 m2, take two grabs for the benthic macroinvertebrate
collections and composite the sediment into the sieve.
11. Process the grab sample for either benthic community analysis or chemistry/toxicity testing as
described in and in Sections 6.2 and 6.3.
12. Repeat steps 4-8 until all samples are successfully collected. To minimize the chance of sampling
the exact same location twice, the boat engines can be turned periodically to change the drift of
the boat, or additional anchor line can be let out.
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page 59
Acceptable grab
At least 7 cm deep with even surface
Unacceptable grab
Sloping surface
Unacceptable grab
Insufficient volume
Unacceptable grab
Wash-pul
Unacceptable grab
Overfilled
Figure 6-1. Illustration of Acceptable and Unacceptable Grabs for Benthic Community Analysis.
An acceptable grab is at least 7 cm in depth (using a 0.04m2 Van Veen sampler), but not oozing out of the
top of the grab, and has a relatively level surface.
6.2 Benthic Macroiinvertebrate Composition And Abundance
6.2.1 Field Processing of Benthic Macroinvertebrate Samples
Grab samples obtained to assess the benthic macroinvertebrate community are processed
as outlined in Table 6-3.
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page 60
Table 6-3. Processing Procedure for Benthic Macroinvertebrate Samples
1. Measure the depth of the sediment at the middle of the sampler and record the value on the data
sheet. The depth should be >7 cm. Record descriptive information about the grab, such as the
presence or absence of a surface floe, color and smell of surface sediments, and visible fauna on the
data sheet.
2. Dump the sediment into a clean basin and then into a 0.5 mm mesh sieve (1.0 mm mesh in CA, OR,
WA). Place the sieve into a table (sieve box) containing water from the sampling station, a larger
bucket or place over the side of the boat. Agitate the tray in the sieve box thus washing away
sediments and leaving organisms, detritus, sand particles, and pebbles larger than 0.5 mm or 1.0 mm
where relevant. This method minimizes mechanical damage to fauna that is common when forceful
jets of water are used to break up sediments. A gentle flow of water over the sample is acceptable.
Extreme care must be taken to assure that no sample is lost over the side of the sieve.
3. Drain the water from the sieve box and gently rinse the contents of the tray to one edge. Remove
large non-living items such as rocks and sticks after inspecting them and ensuring that all benthic
organisms are included in the collection. Using either your fingers or a spoon, GENTLY scoop up the
bulk of the sample and place it in the 1 L Nalgene screw-top bottle (which should be placed in the
sieve or a bucket in case some of the sample spills over).
4. Rinse the outside of the sample jar into the sieve, then, using a funnel, rinse the contents into the jar.
The jar should be filled no more than one-half full. If the quantity of sample exceeds 500 ml, place
the remainder of the sample in a second container with a "2 of 2" label. For samples with a large
amount of benthos, additional jars may be needed.
5. Be sure to place the sample and jar number on a waterproof label and place inside the sample
container. Record the total number of jars on the Sample Collection Form (Figure 6-2).
6. Carefully inspect the sieve to ensure that all organisms are removed. Use fine forceps (if necessary)
to transfer fauna from the sieve to the bottle containing the proper sample number.
7. 100% percent buffered formalin is used to fix and preserve benthic samples. A 100 % buffered,
stained stock formalin solution should be mixed according to the directions in Table 3-2. 100 ml of
the formalin should be added to each sample jar along with an additional teaspoon-full of borax is to
ensure saturation of the buffer.. FILL THE JAR TO THE RIM WITH SEAWATER TO ELIMINATE ANY
AIR SPACE. This eliminates the problem of organisms sticking to the cap because of sloshing during
shipment. Teams may choose to use a more dilute formalin solution in larger quantities as long as
the end concentration of the preservative is between 6 and 7 percent.
8. Use a pencil to fill out waterproof benthos label(s) with the pertinent sample information and place it
inside the bottle(s).
9. Seal the lid with electrical tape. If the sample occupies more than one container, label all the sample
bottles containing material from that grab together. Each benthos jar from a single site will have the
same sample ID number. Gently rotate the bottle to mix the contents and place in the dark.
10. Prior to sieving the next sample, use copious amounts of forceful water and a stiff brush to clean the
sieve, thereby minimizing cross-contamination of samples.
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page 61
NCCA2010 SAMPLE COLLECTION FORM - (Back)
SITE ID: NCCA10 LAOOCO DATE: O4>/O I./. 2,ฐ.1.0.
BENTHIC INFAUNA COLLECTION No sampi. coBBctKi Q
GRAB AREA (m1): ฃ
.05
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SIEVE SIZE: 0.5 mm O 1.0 mm
q q q I 05
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1 2.
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3 TYPE: _.....-._ O Other:
+ Standard Ponar
NOTE:
NUMBER OF GRABS: 1 O 2 * Qnb> we nxjuired forumpten leutliiui 0.03 m'
Ptwerved Commsntt
/^
SEDIMENT CHARACTERISTICS (Benthic Grab) ^ V ^
COLOR: O Black O Brawn O Light Brown Dark Brown O Gray O Oth^^^ #s j*
& ^ n&ป&
SEtflMEhT GRAIN SIZE fNalnene 125ml) No Sample Codectod O
Sample ID
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Sample Voluinc I *-e,^J
(T*fBปtซ 100 mL) -A,QS>i(t-il
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y'V SEDIMENT TOC {Nalwne 60ml) No sปnpiซ CoMซปd Q
Sample ID
.^3 .9. 1. oft.
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Comments
V g * SEDIMENT TOXICITY (1 gal Screw Top Bucket) Ho Sample Collected O
<:
Sample ID
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3003052621
Figure 6-2. Example Sample Collection Form (Back)
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
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6.3 Sediment Composition, Chemistry And Toxicity
In addition to grab samples collected for benthic community analysis, additional grabs are
collected for chemical analyses (organics/metals and TOC), grain size determination, and for
use in acute toxicity tests. The top two centimeters of these grabs are removed, homogenized,
and split into these four sample types.
6.3.1 Field Processing of Sediment Samples for Chemistry and Toxicity
Testing
Because of contamination concerns, these samples are removed and processed in the
order described below in Table 6-4.
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Field Operations Manual Date: April 23, 2010
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Table 6-4. Processing Procedure for Sediment Composition, Chemistry and Toxicity
Testing
1. As each grab is retrieved, carefully examine it to determine acceptability. The grab is considered
acceptable as long as the surface layer is intact. The grab need not be greater than 7 cm in depth for
chemistry samples, but the other criteria outlined above apply. Carefully drain off, or siphon, any
overlying water, and remove and discard large, non-living surface items such as rocks or pieces of
wood. Remove any submerged aquatic vegetation (SAV) after recording its presence on the field data
sheet.
NOTE: Great care must be taken to avoid contamination of this sample from atmospheric contaminants.
The boat engine should be turned off or the boat maneuvered to ensure the exhaust is down wind. All
containers, including the grab sampler, should be kept closed except for when opening is necessary to
remove or add samples.
2. A clean stainless steel or Teflon spoon is used to remove sediments from grab samples for these
analyses. The stainless steel or Teflon spoon must be washed with Alconox and rinsed with ambient
seawater or lake water before use in obtaining grab samples.
3. Remove the top two cm of sediment using the stainless steel or Teflon spoon. Sediment which is in
direct contact with the sides of the sampler should be excluded as they may be contaminated from
the device. Place the sediment in a stainless steel pot or bowl and place the pot in a cooler on wet ice
(NOT dry ice). The sample must be stored at 4ฐC, NOT FROZEN.
4. Repeat obtaining sediment samples from the grab and compositing the sediment in the same
stainless pot until a sufficient quantity of sediment has been collected for all samples (approximately
4L). Stir sediment homogenate after every addition to the composite to ensure adequate mixing.
Keep the container covered and in the cooler between grabs.
5. Homogenize the sediment by stirring with a Teflon paddle or stainless steel spoon for 10 minutes.
Divide the composite into the following four sample types.
6. ORGANICS and METALS - Using a stainless steel spoon, carefully place 250 ml of sediment in a
500 ml glass bottle for chemical analysis. CARE MUST BE TAKEN TO ENSURE THAT THE INSIDE
OF THE BOTTLE, BOTTLE CAP, AND THE SAMPLE IS NOT CONTAMINATED. Record the sample
number, wrap the jar in "bubble wrap" to protect it from breakage, and place the sample on wet ice
(NOT dry ice). To reduce the possibility of breakage, the sample should be stored at 4ฐC, NOT
FROZEN.
7. SEDIMENT GRAIN SIZE - Using a stainless steel spoon, place approximately 100 mL of sediment
into a clean 125 mL Nalgene sampling jar. Record the sample number and keep on ice at 4ฐC. Store
this sample on wet ice (NOT dry ice).
9. TOTAL ORGANIC CARBON - Using a stainless steel spoon, place approximately 50 mL of sediment
into a pre-cleaned 60 mL Nalgene sampling jar. Record the sample number and keep on wet ice at
4ฐC.
10. SEDIMENT TOXICITY - Using the stainless steel spoon, fill approximately 75-85% of 1 gallon plastic
bucket for toxicity testing with sediment (minimum volume required is 3000 mL). Record the sample
number and place the sample on wet ice (NOT dry ice). The sample must be stored at 4ฐC, NOT
FROZEN.
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Field Operations Manual Date: April 23, 2010
Page 64
7.0FISH TISSUE COLLECTION
Fish will be collected at all NCCA sites to be analyzed for whole body concentrations of
organic and inorganic contaminants to generate data for ecological purposes ("eco" fish tissue
samples). Results will be used to evaluate ecological risks associated with fish consumption by
wildlife.
An additional fish tissue sample for human health contaminant analysis will be taken at 150
Great Lakes sites. Refer to section 7.2 for detailed information regarding this sample.
7.1 Ecological Contamination Fish Collection
Ecological fish tissue collection will be based on biogeographically specific "target species"
lists developed for each of the regional areas- Great Lakes, Northeast, Southeast, Gulf, and
West Coast. In the event that target species cannot be caught at a site, then species of similar
habit/habitat may be substituted. All attempts should be made to collect the targeted species.
Teams are not required to expend any more than 3 hours in attempting to collect the ecological
fish tissue sample. Teams may, however, spend additional time fishing if desired.
Any reasonable method which represents the most efficient or best use of the available time
on station may be used to collect the fish (e.g., otter trawl, hook and line, gill net, seine, etc.). It
is not recommended that specimens be obtained by purchasing fish dockside unless it can be
documented that the fish purchased came from an area in close proximity to the X-site (i.e.
within 500 meters). Record pertinent information regarding the fish collection method, start and
stop times, and fishing location on the Eco Fish Collection Form, side 1 (Figure 7-1).
Specimens collected should be identified to species and measured to the nearest millimeter
(total length). Record the taxonomic name (genus-species) and the length of each fish on the
Eco Fish Collection Form, side 2 (Figure 7-2). The minimum length for a specimen for ecological
risk purposes is 100 mm with a preferred length of 100 - 400 mm. A minimum of 5 individuals
should be collected for the composite sample. All individuals must be of similar size, such that
the smallest individual in the composite is no less than 75% of the total length of the largest
individual. Up to 20 individuals (a total of 500 g of whole body tissue is needed) should be
collected and retained for analysis. If it is suspected that 20 individuals will yield less than 500 g
total weight, additional specimens should be collected. The lengths of any additional fish should
be recorded on a supplemental fish collection form and submitted along with the Eco Fish
Collection Form.
7.1.1 Equipment and Supplies for Eco Fish Tissue Sampling.
Table 7-1 lists the equipment and supplies necessary for field crews to collect ecological fish
tissue samples. This list is comparable to the checklist presented in Appendix A, which provides
information to ensure that field teams bring all of the required equipment to the site. Additional
Eco Fish Collection Supplies can be ordered from GLEC at 231-941-2230.
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National Coastal Condition Assessment
Field Operations Manual
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Page 65
Table 7-1. Equipment and SuppliesEco Fish Tissue Collection
For collecting fish
composite sample
Scientific collection permit
Otter trawl (or other device to collect
sufficient sample)
Sampling vessel (including boat, motor,
trailer, oars, gas, and all required safety
equipment)
Coast Guard-approved personal
floatation devices
Global Positioning System (GPS)
unit
Livewell and/or buckets
Measuring board (millimeter
scale)
Clean nitrile gloves
Wooden bat
For storing and
preserving fish
composite sample
2 gallon plastic self-sealing bags
Large plastic (composite) bags
Coolers
Plastic cable ties
Dry ice or wet ice (for temporary
transport)
For documenting the
fish composite sample
Field Record Forms
Clipboard
#2 pencils
Sample Identification Labels
Tyvek label tags
Fine tipped indelible markers
For shipping the fish
composite samples
Preaddressed FedEx airbill
Coolers
Dry ice (50 Ibs per cooler)
Tracking Form
Packing/strapping tape
7.1.2 Sampling Procedure
The eco fish tissue samples will be collected using any reasonable method that is most
efficient and the best use of available time on station. Fish tissue sample collection occurs in
proximity to the X-site where other indicator samples are obtained (within a 500 meter radius of
the X-site). Record the method(s) used on the Eco Fish Collection Form.
At least five individuals of the target species are needed, yielding a minimum of 500 g total
weight. If a full composite sample is not collected after 3 hours of effort, teams may terminate
the sampling and submit as many fish as possible. Record the details of the sample on the Eco
Fish Collection Form. If the target species are unavailable, the fisheries biologist will select an
alternative species (i.e., a species that is commonly present in the study area, with specimens
of harvestable or consumable size, and in sufficient numbers to yield a composite) to obtain a
fish composite sample from the species that are available. Recommended target species are
given in Tables 7-2 and 7-3.
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Field Operations Manual
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Table 7-2. Recommended Great Lakes Target Species for Whole Body Fish Tissue Collection
by Lake
Lake
Erie
Lake
Huron
Lake
Superior
Lake Ontario
Lake
Michigan
Family name
Cyprinidae
Gobiidae
Ictaluridae
Moronidae
Percidae
Sciaenidae
Centrarchidae
Cottidae
Percidae
Osmeridae
Salmonidae
Catostomidae
Centrarchidae
Cottidae
Cyprinidae
Esocidae
Gasterosteidae
Gobiidae
Ictaluridae
Lotidae
Moronidae
Percidae
Percopsidae
Salmonidae
Sciaenidae
Centrarchidae
Cottidae
Cyprinidae
Gobiidae
Lotidae
Percidae
Salmonidae
Common name
Common carp
Round goby
Channel catfish
White perch
White bass
Yellow perch
Walleye
Freshwater drum
Smallmouth bass
Slimy sculpin
Yellow perch
Walleye
American / Rainbow smelt
Lake whitefish
Cisco/ Lake Herring
Lake trout
Shorthead redhorse
Rock bass
Pumpkinseed
Bluegill
Smallmouth bass
White crappie
Black crappie
Mottled sculpin
Slimy sculpin
Common carp
Lake chub
Bluntnose minnow
Northern pike
Muskellunge
Three-spined stickleback
Round goby
Tubenose goby
Brown bullhead
Stonecat
Channel catfish
Burbot
White perch
White bass
Ruffe
Yellow perch
Logperch
Sauger
Walleye
Trout-perch
Pink salmon
Coho salmon
Rainbow trout
Lake whitefish
Chinook salmon
Lake trout
Freshwater drum
Rock bass
Pumpkinseed
Bluegill
Mottled sculpin
Slimy sculpin
Lake chub
Bluntnose minnow
Round goby
Tubenose goby
Burbot
Yellow perch
Logperch
Lake whitefish
Lake trout
Scientific name
Cyprinus carpio
Neogobius melanostomus
Ictalurus punctatus
Morone amehcana
Morone chrysops
Perca flavescens
Sander vitreus
Aplodinotus grunniens
Micropterus dolomieu
Cottus cognatus
Perca flavescens
Sander vitreus
Osmerus mordax
Coregonus clupeaformis
Coregonus Artedi
Salvelinus namaycush
Moxostoma macrolepidotum
Ambloplites rupestris
Lepomis gibbosus
Lepomis macrochirus
Micropterus dolomieu
Pomoxis annularis
Pomoxis nigromaculatus
Cottus bairdii
Cottus cognatus
Cyprinus carpio
Couesius plumbeus
Pimephales notatus
Esox lucius
Esox masquinongy
Gasterosteus aculeatus aculeatus
Neogobius melanostomus
Proterorhinus marmoratus
Ameiurus nebulosus
Noturus flavus
Ictalurus punctatus
Lota lota
Morone amehcana
Morone chrysops
Gymnocephalus cernuus
Perca flavescens
Percina caprodes
Sander canadensis
Sander vitreus
Percopsis omiscomaycus
Oncorhynchus gorbuscha
Oncorhynchus kisutch
Oncorhynchus mykiss
Coregonus clupeaformis
Oncorhynchus tshawytscha
Salvelinus namaycush
Aplodinotus grunniens
Ambloplites rupestris
Lepomis gibbosus
Lepomis macrochirus
Cottus bairdii
Cottus cognatus
Couesius plumbeus
Pimephales notatus
Neogobius melanostomus
Proterorhinus marmoratus
Lota lota
Perca flavescens
Percina caprodes
Coregonus clupeaformis
Salvelinus namaycush
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National Coastal Condition Assessment
Field Operations Manual
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Table 7-3. Recommended Marine Target Species for Whole Body Fish Tissue Collection by
Specific Biogeographical Region
Northeast
Southeast/
Gulf of
Mexico
West Coast
Family name
Ictaluridae
Moronidae
Paralichthyidae
Pleuronectidae
Sciaenidae
Sparidae
Nephropoidea
Ariidae
Paralichthyidae
Sciaenidae
Sparidae
Atherinopsidae
Cottidae
Cynoglossidae
Embiotocidae
Gasterosteidae
Paralichthyidae
Pleuronectidae
Sciaenidae
Serranidae
Common name
White catfish
Channel catfish
White perch
Summer flounder
Winter flounder
Gray weakfish
Scup
Lobster
Hardhead sea catfish
Gafftopsail sea catfish
Southern flounder
Gulf Plunder
Summer flounder
Sand weakfish (or seatrout)
Spot croaker
Gray weakfish
Atlantic croaker
Speckled Trout
Red Drum
Pinfish
Topsmelt silverside
Pacific staghorn sculpin
Saddleback sculpin
California tonguefish
Shiner perch
Striped sea perch
Three-spined stickleback
Pacific sanddab
Speckled sanddab
California flounder
Butter sole
English sole
Starry flounder
Pacific sand sole
White croaker
Spotted sand bass
Barred sand bass
Scientific name
Ameiurus catus
Ictalurus punctatus
Morone americana
Paralichthys dentatus
Pseudopleuronectes amehcanus
Cynoscion regalis
Stenotomus chrysops
Homarus americanus
Ahopsis felis
Bagre marinus
Paralichthys lethostiqma
Paralichthys albigutta
Paralichthys dentatus
Cynoscion arenarius
Leiostomus xanthurus
Cynoscion regalis
Micropogonias undulatus
Cynoscion nebulosus
Sciaenops ocellatus
Lagodon rhomboides
Atherinops affinis
Leptocottus armatus
Oligocottus rimensis
Symphurus atricaudus
Cymatogaster aggregata
Embiotoca lateralis
Gasterosteus aculeatus aculeatus
Citharichthys sordidus
Citharichthys stigmaeus
Paralichthys californicus
Isopsetta isolepis
Parophrys vetulus
Platichthys stellatus
Psettichthys melanostictus
Genyonemus lineatus
Paralabrax maculatofasciatus
Paralabrax nebulifer
The procedures for collecting and processing fish composite samples are presented in
Table 7-4.
Table 7-4. Sampling Procedure for Eco Fish Tissue Composite Samples
1. Put on clean nitrile gloves before handling the fish. Do not handle any food, drink, sunscreen, or
insect repellant until after the composite sample has been collected, measured, and bagged.
2. Rinse potential target species/individuals in ambient water to remove any foreign material from the
external surface and placed in clean holding containers (e.g., livewells, buckets)..
3. The eco fish composite must consist of at least 5 fish of adequate size to provide a total weight of
500 grams of whole-body tissue. Select fish for the composite based on the following criteria:
all are of the same species;
all are of similar size, so that the smallest individual in a composite is no less than 75% of the
total length of the largest individual; and
all are collected at the same time, i.e., collected as close to the same time as possible, but no
more than one week apart (Note: individual fish may have to be frozen until all fish to be
included in the composite are available for delivery to the designated laboratory).
4. Identify the fish to species and record the scientific name of the Fish Tissue Data Form (Figure 7-
2). Accurate taxonomic identification is essential in assuring and defining the organisms that have
been composited and submitted for analysis. Individuals from different species should not be used
in a single sample.
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page 68
Table 7-4. Sampling Procedure for Eco Fish Tissue Composite Samples
5. Measure each individual fish to determine total body length. Measure total length of each specimen
in millimeters, from the anterior-most part of the fish to the tip of the longest caudal finray (when the
lobes of the caudal fin are depressed dorsoventrally).
6. Record collection method, sample number, species retained, specimen lengths, location collected
and sampling date and time on the Fish Collection Form (Figure 7-1). Make sure the sample ID
numbers recorded on the collection form match those on the sample labels.
7. Remove each fish retained for analysis from the clean holding container(s) (e.g., livewell) using
clean nitrile gloves. Dispatch larger fish using a clean wooden bat (or equivalent wooden device).
8. Place each fish in a 2 gallon self-sealing bag. All fish from the composite sample should be placed
in the same bag. Be careful offish with spines that may pierce the bag. If spines are likely to
puncture the bag, break off or clip the spines with a clean side-cutter or other appropriate tool and
place the spine in the bag with the fish. If all the fish collected will not fit in a single 2 gallon bag,
use additional bags as necessary.
9. Prepare interior and exterior Sample Identification Labels for the 2 gallon bag(s), ensuring that the
label information matches the information recorded on the Fish Collection Form. Be sure to
include fish species and maximum and minimum lengths on the labels. Place the interior
label inside a small (sandwich size) self-sealing bag and place it inside the 2 gallon bag with the
fish composite. Affix the exterior label to the 2 gallon bag and cover with clear plastic tape. If
additional 2 gallon bags are used, fill out extra labels with the same sample ID and information for
each bag and label accordingly (i.e. bag 2 of 2).
10. Double-bag the entire set of specimens in the composite, that is, place all the 2 gallon bags in the
composite from the site inside a large plastic bag.
11. Prepare a Sample Identification Label for the outer bag, ensuring that the label information
matches the information recorded on the Fish Collection Form. Be sure to include fish species
and maximum and minimum lengths on the label. Affix the sample label to a Tyvektag and
cover with clear plastic tape. Thread a cable tie through the grommet in the Tyvek tag and seal the
outer bag with the cable tie.
12. After the sample is packaged, place it immediately on dry ice for shipment. If samples will be
carried back to a laboratory or other facility to be frozen before shipment, wet ice can be used to
transport bagged fish samples in the coolers to a laboratory or other interim facility.
13. Samples may be stored on dry ice for a maximum of 24 hours. You have the option, depending on
site logistics, of:
shipping the samples packed on sufficient quantities of dry ice (50 pounds minimum, layered to
ensure direct contact between fish and dry ice) to keep samples frozen for up to 48 hours, via
priority overnight delivery service (e.g., Federal Express), so that they arrive at the sample
preparation laboratory within less than 24 hours from the time of sample collection, or
freezing the samples within 24 hours of collection at <-20ฐC, and storing the frozen samples
until shipment within 2 weeks of sample collection (frozen samples will subsequently be
packed on at least 50 pounds of layered dry ice and shipped to the sample preparation
laboratory via priority overnight delivery service).
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page 69
NCCA 2010 ECO FISH COLLECTION (Front)
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page 70
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The eco fish corn'ppsjfe must consist of at least 5 fish of adequate size to provide a total weight of 500 grams of wtiole-body tissue.
9233044667
03/31/2010 NCCA ECO Fish Colteclion (Back)
Figure 7-2. Example Eco Fish Collection Form (Back)
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page 71
7.2 Summary Of Method For Human Health Fish Tissue Sampling
Human health fish composites will be collected at a subset of 150 of the Great Lakes sites
(30 sites per lake), and fillet tissue will be analyzed for mercury, fatty acids, and contaminants of
emerging concern (e.g., perfluorinated compounds or PFCs). This section contains the sampling
procedures and target species for human health fish tissue collection. Note that the human
health fish species table (Table 7-6) includes 26 priority target species and 18 alternative fish
species. Field crews should attempt to collect a priority target species wherever possible. If
priority target species are not available at a particular site, then the field crew should collect a
composite of one of the alternative fish species. In the event that a team is unable to collect fish
which are on the human health species list, then the field crew should contact either Leanne
Stahl, Great Lakes Human Health Fish Tissue Study Manager (U.S. EPA Office of Water), at
202-566-0404 or Elaine Snyder, Tara Kolodiej or Carolina Gallardo of Tetra Tech, Inc. at 410-
356-8993 for further direction.
Any reasonable method which represents the most efficient or best use of the available time
on station may be used to collect the fish (e.g., gill net, otter trawl, or hook and line).
Purchasing fish is not an option for human health fish tissue collection. Record sample
collection information on the Human Health Fish Collection Form, side 1 (Figure 7-3).
Specimens collected for each composite should be identified using scientific names (genus
and species). Record the scientific name on the Human Health Fish Collection Form, side 2
(Figure 7-4), along with the total length (to the nearest mm) for each specimen in the composite.
Human health fish composites should consist of 5 similarly sized (i.e., the total length of the
smallest specimen is no less than 75% of the total length of the largest specimen) adult fish of
the same species that will collectively yield about 500 g of fillet tissue.
Table 7-5 lists the equipment and supplies necessary for field crews to collect human health
fish tissue samples. Additional Eco Fish Collection Supplies can be ordered from Tetra Tech at
410-356-8993. A list of frequently asked questions and responses will be provided with the fish
sampling supplies to clarify situations that field crews may encounter while collecting human
health fish composites. The procedures for collecting and processing fish composite samples
are presented in Table 7-7.
Table 7-5. Equipment and SuppliesHuman Health Fish Tissue Collection
For collecting fish
composite sample
Scientific collection permit
Otter trawl (or other device to collect
sufficient sample)
Sampling vessel (including boat, motor,
trailer, oars, gas, and safety equipment)
Clean nitrile gloves
Coast Guard-approved personal
floatation devices
Global Positioning System (GPS)
Livewell and/or buckets
Measuring board (millimeters)
Wooden bat
For storing and
preserving fish
composite sample
Solvent rinsed aluminum foil
Food-grade poly tubing
Large plastic (composite) bags
Coolers
Plastic cable ties
Dry ice or wet ice (for temporary
transport)
For documenting the
fish composite sample
Field Record Forms
Clipboard
#2 pencils
Sample Identification Labels
Tyvek label tags
Fine tipped indelible markers
For shipping the fish
composite samples
Preaddressed FedEx airbill
Coolers
Dry ice (50 Ibs per cooler)
Tracking Form
Packing/strapping tape
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page 72
Table 7-6 Target Fish Species for Great Lakes Human Health Fish Tissue Study Fillet Composites
Priority Target Fish Species
Family Name
Centrarchidae
Cyprinidae
Esocidae
Ictaluridae
Lotidae
Moronidae
Percidae
Salmonidae
Sciaenidae
Common Name
Rock bass
Smallmouth bass
Largemouth bass
White crappie
Black crappie
Common carp
Northern pike
Muskellunge
Chain pickerel
Channel catfish
Burbot
White perch
White bass
Yellow perch
Sauger
Walleye
Lake whitefish
Pink salmon
Coho salmon
Chinook salmon
Rainbow trout
Atlantic salmon
Brown trout
Lake trout
Freshwater drum
Scientific Name
Ambloplites rupestris
Micropterus dolomieu
Micropterus salmoides
Pomoxis annularis
Pomoxis nigromaculatus
Cyprinus carpio
Esox lucius
Esox masquinongy
Esox niger
Ictalurus punctatus
Lota lota
Morone americana
Morone chrysops
Perca flavescens
Sander canadensis
Sander vitreus
Coregonus clupeaformis
Oncorhynchus gorbuscha
Oncorhynchus kisutch
Oncorhynchus tshawytscha
Oncorhynchus mykiss
Salmo salar
Salmo trutta
Salvelinus namaycush
Aplodinotus grunniens
Alternative Fish Species
Family Name
Catostomidae
Centrarchidae
Ictaluridae
Salmonidae
Common Name
Quillback
Longnose sucker
White sucker
Northern hog sucker
Bigmouth buffalo
Black buffalo
Green sunfish
Pumpkinseed
Warmouth
Bluegill
Longear sunfish
Black bullhead
Yellow bullhead
Brown bullhead
Cisco
Bloater
Round whitefish
Brook trout
Scientific Name
Carpiodes cyprinus
Catostomus catostomus
Catostomus commersonii
Hypentelium nigricans
Ictiobus cyprinellus
Ictiobus niger
Lepomis cyanellus
Lepomis gibbosus
Lepomis gulosus
Lepomis macrochirus
Lepomis megalotis
Ameiurus melas
Ameiurus natalis
Ameiurus nebulosus
Coregonus artedi
Coregonus hoyi
Prosopium cylindraceum
Salvelinus fontinalis
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page 73
Table 7-7. Sampling Procedures for Human Health Fish Tissue Composite Samples
1. Put on clean nitrile gloves before handling the fish. Do not handle any food, drink, sunscreen, or
insect repellant until after the composite sample has been collected, measured, and wrapped.
2. Rinse potential target species/individuals in ambient water to remove any foreign material from the
external surface and placed in clean holding containers (e.g., livewells, buckets).
3. The composite should consist of 5 fish of adequate size to provide a total of 500 grams of fillet tissue
for human health samples. Select fish for each composite based on size similarity and priority target
species or alternative fish species in Table 7-5.
Accurate taxonomic identification is essential in assuring and defining the organisms that have been
submitted for analysis. Individuals from different species should not be used in a single sample.
4. Measure each individual fish to determine total body length. Measure total length of each specimen
in millimeters, from the anterior-most part of the fish to the tip of the longest caudal fin ray (when the
lobes of the caudal fin are depressed dorsoventrally).
5. On the Human Health Fish Collection Form, side 2 (Figure 7-4), record the sample identification
number and response to length and species question in the header of the form. Below the header,
record species retained, specimen length (total length in mm), and any relevant comments. Extra
rows are provided on the form in the event that additional specimens are collected to meet the 500
gram fillet tissue requirement (refer to Frequently Asked Questions for further clarification). Make
sure the sample ID and specimen numbers recorded on the form match those on the sample labels.
6. Remove each fish retained for analysis from the clean holding container(s) (e.g., livewell) using
clean nitrile gloves. Dispatch each fish using a clean wooden bat (or equivalent wooden device).
7. Wrap each fish in extra heavy-duty aluminum foil, with the dull side in (foil provided by EPA as
solvent-rinsed, oven-baked sheets).
8. Prepare a Sample Identification Label for each sample, ensuring that the label information matches
the information recorded on the Human Health Fish Tissue Sample form. Be sure to include fish
species and specimen length on each label.
9. Cut a length of food grade tubing (provided by EPA) that is long enough to contain each individual
fish and to allow extra length on each end to secure with cable ties. Place each foil-wrapped
specimen into the appropriate length of tubing. Seal each end of the tubing with a plastic cable tie,
and attach the appropriate Sample Identification Label to the plastic tubing using clear tape
(wrapping completely around the wrapped fish so that the clear tape wraps over itself).
10. Double-bag the entire set of specimens in the composite, that is, place all the fish in the composite
from the site inside a large plastic bag.
11. Prepare a Sample Identification Label for the outer bag, ensuring that the label information matches
the information recorded on the Fish Collection Form. Be sure to include fish species and
lengths on the label. Affix the sample label to a Tyvektag and cover with clear plastic tape. Thread
a cable tie through the grommet in the Tyvek tag and seal the outer bag with the cable tie
12. As each sample is packaged, place it immediately on dry ice for shipment. If samples will be carried
back to a laboratory or other facility to be frozen before shipment, wet ice can be used to transport
wrapped and bagged fish samples in the coolers to a laboratory or other interim facility.
13. If possible, keep all specimens designated for a particular composite in the same shipping container
(ice chest) for transport.
14. Samples may be stored on dry ice fora maximum of 24 hours. You have the option, depending on
site logistics, of:
shipping the samples packed on sufficient quantities of dry ice (50 pounds minimum, layered to
ensure direct contact between fish and dry ice) to keep samples frozen for up to 48 hours, via
priority overnight delivery service (e.g., Federal Express), so that they arrive at the sample
preparation laboratory within less than 24 hours from the time of sample collection, or
freezing the samples within 24 hours of collection at <-20ฐC, and storing the frozen samples until
shipment within 2 weeks of sample collection. Frozen samples will subsequently be packed on
at least 50 pounds of layered dry ice and shipped to the sample preparation laboratory via
priority overnight delivery service.
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page 74
NCCA2010 HUMAN HEALTH FISH COLLECTION (Front) ซ"ปซ"ป<*"*>:
JfiS
SITEID: NCCAGL10
DATE: ^ k /.O.I ./ 2 . ฐ . 1 . ฐ .
Collection Method
;eiu.NET \
O OTHER
v. (,
Trawl/Seine Start:
LATITUDE:
Decimal Degrwt
RAGNETIC:
LONGITUDE:
START TIME:
Trawl/Seine End:
LATITUDE:
Decimal D*graM
If Seine: LENGTH:
(m)
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FLAG:
Flag Codes: K = no measurement made; U = %ggedweBiErement; FI. F2. etc. = ซags assigned by each field crew. Explain all Hags in comments section.
Flag
Comments
. 03^31/2010 NCCA Human Health Fish Collection (Front)
Figure 7-3. Example Human Health Fish Tissue Data Form (Front)
5721053452
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Field Operations Manual
Date: April 23, 2010
Page 75
NCCA2010 HUMAN HEALTH FISH COLLECTION (Back)
,,.w,Jf*
SITE ID; NCCAGL10
DATE: O 4? / 0 I A2.0.1.0. PAฐE: * OF
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(refer to Frequently Asked Questions for possible exceptions). S ^ *
03/31/2010 NCCA Human Health Fish Cotlectico (Back)
Figure 7-4. Example Human Health Fish Tissue Data Form (Back)
7461152602
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Field Operations Manual
Date: April 23, 2010
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8.0FINAL SITE ACTIVITIES
Prior to leaving the site, make a general visual assessment of the site and its adjacent
shoreline. The objective of the site assessment is to record observations of the shoreline and
site characteristics that are useful for future data interpretation, ecological value assessment,
development of associations, and verification of stressor data. Your observations and
impressions are extremely valuable.
You will filter and process the fecal indicator and chlorophyll-a samples, and collect the
dissolved nutrients sample from the chlorophyll-a filtrate. You will also conduct a final check of
the data forms, labels and samples. The purpose of the second check of data forms, labels and
samples is to assure completeness of all sampling activities. Finally, clean and pack all
equipment and supplies, and clean the launch site and staging areas. After you leave the site,
report the sampling event to the Information Management Coordinator, and ship or store the
samples. Activities described in this section are summarized in Figure 8-1.
COMPLETE SITE
ASSESSMENT
(4 People)
REVIEW DATA FORMS
(Crew Leader)
Completeness
Accuracy
Legibility
Flags/Comments
REVIEW SAMPLE LABELS
(Crew Leader)
Completeness
Accuracy
Legibility
Cross-check with forms
PACK EQUIPMENT AND
SUPPLIES FOR TRANSPORT
(2 People)
FILTER, PRESERVE, &
INSPECT SAMPLES
(3 People)
Complete
Sealed
Ice packs
Packed for transport
INSPECT BOAT, MOTOR,
TRAILER, AND NETS FOR
PRESENCE OF PLANT AND
ANIMAL MATERIAL, AND
CLEAN THOROUGHLY
(3 People)
LOAD BOAT ONTO TRAILER;
CLEAN UP LAUNCH SITE
AND STAGING AREA
(2 People)
LEAVE SITE
COMMUNICATIONS
* SHIP SAMPLES
Figure 8-1. Final Site Activities Summary.
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Field Operations Manual Date: April 23, 2010
Page 77
8.1 General Site Assessment
Complete the Site Assessment Form (Figure 8-2) after sampling, recording all observations
from the site that were noted during the course of the visit. This Site Assessment Form is
designed as a template for recording pertinent field observations. It is by no means
comprehensive, and any additional observations should be recorded in the General Assessment
section.
8.1.1 Shoreline Activities and Disturbances
Record shoreline activities and disturbances on a rating of low, moderate or high. For this
portion of the site assessment, consider the shoreline adjacent to the sampling site that is
visible from the X-site. Consider only the shoreline which is in the same estuary, waterbody
and/or embayment as the X-site. Using your best judgment, direct the assessment to the
shoreline that would be considered ecologically significant to the sampling site. If the shore
cannot be seen from the X-site (due to weather conditions or distance) note in the comments
section the reason that the shoreline assessment was not possible.
8.1.2 Site Characteristics
Record observations regarding the general characteristics of the site on the Site
Assessment Form. When assessing these characteristics, look at a 200 m radius around the X-
site. Rank the site between "pristine" and "highly disturbed", and between "appealing" and
"unappealing" on a scale of 1 to 5. As with other aspects of the general visual assessment, all
crew members should provide input into the final ranking. These observations will be
understandably subjective, but provide valuable information on crew impressions of the overall
character of the site that can be used by NCCA analysts to help explain data. Document any
signs of pipe outflows or shoreline enhancement or retention. Document the weather conditions
on the day of sampling, and any extreme weather conditions just prior to sampling.
8.1.3 General Assessment
Record any additional information and observations in this narrative section. Information to
include could be observations on biotic integrity, presence of SAV, presence and abundance of
endangered and/or exotic species, local anecdotal information, or any other pertinent
information about the site or its adjacent areas. Record any observations that may be useful for
future data interpretation.
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page 78
NCCA 2010 SITE ASSESSMENT (Front)
SITE ID: NCCA10 LAOOQO
DATE:
/Q I ./.
SHORELINE ACTIWTIES AND DISTURBANCES OBSERVED
(Intensity: Btonk=Not obwrved, LvLow, M=*taderat9, M=Heaw)
Residential
Recreational
Agricultural
Industrial
Management
L M H
L M H
L M H
L M H
L M H DWTVIIM
L M H Roadi
L M H
H SซwlflซT
H HlklngTralll
H Partปp Campground*
H Ptlmlt>iปPปrt.a, Camping
H rrumitur
H SurbcaFllim
H Oimai
M H Cropland
M H Putin
M H ljvซซloctu.ซ
M H Orchard!
M H Poultry
H H Irrigation Equip.
M H WltwWItrtdrawtl
Water body
Character
Dominant
Land Use
SITE CHARACTERISTICS (200 m radius)
Pristine
Appealing
O5
O5
O4
4
3
O3
Dominant Land Use
O Forest
O Agriculture O Ral1
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Highly Disturbed
Unappealing
O SuburbanfTown
WEATHER
t-Esst-rMfl \ FOOT
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GENERAL ASSESSMENT (Biotic ii^.'tily^'egeutlon diversity, Local anecdotal information)
tS
TO
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SHE.
is SOFT
ThE ECO FISH SAMPLE UOE CO(JLฃCTE3> Z
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^^ 03/11/2010 NCCA Site Assessment
Figure 8-2. Example Site Assessment Form.
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Field Operations Manual
Date: April 23, 2010
Page 79
8.2 Processing The Fecal Indicator And Chlorophyll-^ Samples
8.2.1 Equipment and Supplies (Fecal Indicator)
Table 8-1 provides the equipment and supplies needed for field crews to filter the fecal
indicator sample. The filtering apparatus for this indicator MUST be sterile.
Table 8-1. Equipment and Supplies List for Fecal Indicator Sample
For processing samples
Nitrile gloves
Sterile screw-cap 50 ml tube
Sterile filter holder, Nalgene 145/147
Vacuum pump (electric or hand)
Sterile saline
Whatman 47 mm polycarbonate 0.4 urn sterile filters
Sterile disposable forceps
4 sterile microcentrifuge tubes containing sterile glass beads
(chilled on dry ice during pre-sampling activities)
Sterile 60 X 15 mm Petri dish
Dry ice
Cooler
Field Operations Manual or laminated Quick Reference Guide
For recording
measurements
Sample Collection Form
Soft (#2) lead pencils for recording data on field forms
Fine-tipped indelible markers for filling out sample labels
Fecal Indicator sample labels (4 vial labels and 1 bag label)
Clear tape strips for covering labels
8.2.2 Procedures for Processing the Fecal Indicator Sample
The fecal indicator sample must be filtered before the chlorophyll-a samples, since the
filtering apparatus needs to be sterile for this sample. The procedures for processing the fecal
indicator sample are presented in Table 8-2. The sample must be filtered and frozen within 6
hours of collection.
At revisit sites, a filter blank is prepared prior to filtering the Enterococci sample. Filter
blanks will be prepared at both Visit 1 and Visit 2. Procedures for preparing the filter blank are
presented in Table 8-3.
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Field Operations Manual Date: April 23, 2010
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Table 8-2. Processing ProcedureFecal Indicator Sample
1. Put on nitrile gloves.
2. Set up sample filtration apparatus on flat surface and attach vacuum pump. Set out 50 ml sterile
centrifuge tube, sterile 60 mm Petri dish, 1 bottle of chilled sterile saline, Whatman 47 mm
polycarbonate sterile filter box, and 2 sterile forceps.
3. Aseptically transfer 4 polycarbonate filters from filter box to base of opened Petri dish. Close the filter
box and set aside.
4. Remove cellulose nitrate (CN) filter (the filter with grid design on it) from funnel and discard. Be sure
to leave the support pad in the filter funnel.
5. Load filtration funnel with sterile polycarbonate filter on support pad (shiny side up). Be sure not to
use the blue divider paper as the filter.
6. Shake sample bottle(s) 25 times to mix well.
7. Measure 25 ml of the mixed water sample in the sterile graduated centrifuge tube and pour into filter
funnel.
8. Replace cover on filter funnel and pump to generate a vacuum (do not generate more than 7 inches
of Hg of vacuum ~15 psi). Keep pumping until all liquid is in filtrate collection flask.
9. If the first 25 ml volume passes readily through the filter, add another 25 ml and continue filtration. If
the filter clogs before completely filtering the first or second 25 ml volume, discard the filter and
repeat the filtration using a lesser volume.
10. Pour approx. 10 ml of the chilled sterile saline into the graduated centrifuge tube used for the
sample. Cap the tube and shake 5 times. Remove the cap and pour the rinse into filter funnel to rinse
filter.
11. Filter the rinsate and repeat with another 10 ml of sterile saline.
12. Remove filter funnel from base without disturbing filter. Using sterile disposable forceps remove the
filter (touching only the filter edges) and fold it in half, in quarters, in eighths, and then in sixteenths
(filter will be folded 4 times).
13. Insert filter into chilled filter extraction tube (with beads) open end first (pointy end up). Replace and
tighten the screw cap, insert tube(s) into bubble envelope on dry ice for preservation during transport
and shipping.
14. Record the volume of water sample filtered through the filter (minimum is 25 ml, target is 50 ml) and
the volume of saline rinse each filter was rinsed with on the Sample Collection Form, Side 1. Record
the filtration start time (beginning of first filter) and finish time (end of fourth filter) for the sample.
15. Repeat steps 6 to 15 for the remaining three filters. It is important that the same sample volume be
filtered through each of the 4 filters.
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Page 81
Table 8-3. Processing ProcedureFecal Indicator Filter Blank
Enterococci filter blanks will be prepared at all revisit sites during both visit 1 and visit 2. Prepare the
filter blanks before filtering the coastal sample.
1. Set up sample filtration apparatus using same procedure as used for the sample above. Chill Filter
Extraction tubes with beads on dry ice.
2. Aseptically transfer 4 polycarbonate filters from filter box to base of opened Petri dish. Close filter
box and set aside.
3. Remove cellulose nitrate (CN) filter (the filter with grid design on it) from funnel and discard. Be
sure to leave the support pad in the filter funnel.
4. Load filtration funnel with sterile polycarbonate filter on support pad (shiny side up).
5. Measure 20 ml of the chilled sterile saline in the sterile graduated centrifuge tube and pour into
filter funnel.
6. Replace cover on filter funnel and pump to generate a vacuum (do not generate more than 7 inches
of Hg of pressure). Keep pumping until all liquid is in filtrate collection flask.
7. Remove filter funnel from base without disturbing filter. Using sterile disposable forceps remove the
filter (touching only the filter edges) and fold it in half, in quarters, in eighths, and then in sixteenths
(filter will be folded 4 times).
8. Insert filter into chilled filter extraction tube (with beads) open end first (pointy end up). Replace and
tighten the screw cap, insert tube(s) into bubble envelope on dry ice for preservation during
transport and shipping.
9. Record the filter blank information on the Sample Collection Form.
10. Label the samples as "blank" on the label and field form, and package and submit these samples to
the lab with the standard samples.
11. Repeat steps 4 to 9 for the remaining three 20 ml volumes of sterile saline to be filtered.
8.2.3 Equipment and Supplies (Chlorophyll-sand Dissolved Nutrients Sample)
Table 8-4 provides the equipment and supplies needed to process the chlorophyll-a sample.
Table 8-4. Equipment and Supplies List for Chlorophyll-a and Dissolved Nutrients Processing
For filtering chlorophyll-a
sample
For recording measurements
For sample collection and
preservation
Whatman GF/F 47mm 0.7 micron
filter pads
Filtration apparatus with graduated
filter holder
Vacuum pump (electric or hand)
Sample Collection Form
Sample labels
#2 pencils
50 ml screw-top centrifuge tube
Aluminum foil square
Plastic (electrical) tape
Dl water
Nitrile gloves
Forceps
Graduated cylinders
Fine-tipped indelible
markers
Clear tape strips
Whirl-pak
Cooler with dry ice
250 ml Nalgene bottle
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Field Operations Manual Date: April 23, 2010
Page 82
8.2.4 Procedures for Processing the Chlorophyll-a and Dissolved Nutrients
Sample
The procedures for processing chlorophyll-a and dissolved nutrients samples are presented
in Table 8-5. Whenever possible, sample processing should be done in subdued light, out of
direct sunlight.
Table 8-5. Processing ProcedureChlorophyll-a and Dissolved Nutrients Sample
1. Put on nitrile gloves.
2. Discard any filtrate collected in the filter flask during the filtration of the Enterococci sample and rinse
the flask thoroughly (three times) with Dl water.
3. Rinse the filter funnel three times with Dl water prior to filtration. Rinse graduated cylinders with Dl
water.
4. Use clean forceps to place a Whatman GF/F 47 mm 0.7 micron filter in the graduated filter holder
apparatus (the same apparatus used previously for filtering the Enterococci sample) with the gridded
side of the interfacing down.
5. Remove chlorophyll-a collection bottle from cooler and shake to mix sample. Pour 250 ml of water
into the filter holder, replace the cap, and use the vacuum pump to draw a small portion of the
sample through the filter.
6. Use the first 10-20 ml of filtrate to rinse the inside of the filter flask and discard the rinsate. Replace
the filter flask and continue filtering. Repeat with an additional two rinses of filtered site water.
7. If 250 ml of site water will not pass through the filter, change the filter, rinse the apparatus with Dl
water, and repeat the procedures using 100 ml of site water. Do not exceed 7 inches of Hg of
vacuum -15 psi or a filtration duration of more than 5 minutes for a single sample volume, to
avoid cell damage or loss of contents during filtering.
8. Observe the filter for readily visible color. If there is visible color, proceed; if not, filter additional
aliquots until color is visible on the filter or until a maximum of 2,000 ml have been filtered.
9. After collecting at least 250 ml of filtrate in the filter flask, remove the bottom portion of the
apparatus and pour 250 ml of the filtrate into the 250 ml Nalgene bottle. This filtrate is used for
dissolved nutrient analyses. Complete the label, including salinity (as taken during the in situ
measurements) and affix to the 250 ml Nalgene bottle. Cover with clear plastic tape
10. Record the dissolved nutrients sample information on the Sample Collection Form. Place the sample
on wet ice.
11. After achieving a readily visible stain on the filter, remove the filter from the holder with clean
forceps. Avoid touching the colored portion of the filter. Fold the filter in half, with the colored side
folded in on itself. Place into a 50 ml screw-top centrifuge tube.
12. Complete the label, including volume filtered and affix to the 50 ml screw-top centrifuge tube. Cover
with clear plastic tape. Record the actual sample volume filtered on the Sample Collection Form.
13. Seal the cap of the centrifuge tube with plastic tape.
14. Wrap the 50 ml tube in a foil square and place in a whirl-pak.
15. Place the whirl-pak containing the filter on dry ice.
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Page 83
8.3 Data Forms And Sample Inspection
After the Site Assessment Form is completed, the Field Team Leader reviews all of the data
forms and sample labels for accuracy, completeness, and legibility. The other team members
inspect all sample containers and package them in preparation for transport, storage, or
shipment. Refer to Appendix D for details on preparing samples for shipping.
Ensure that all required data forms for the site have been completed. Confirm that the SITE-
ID, the visit number, and date of visit are correct on all forms. On each form, verify that all
information has been recorded accurately, the recorded information is legible, and any flags are
explained in the comments section. Ensure that written comments are legible, with no
"shorthand" or abbreviations. Make sure there are no stray markings in on the forms. Make sure
the header information is completed on all pages of each form. After reviewing each form, initial
the upper right corner of each page of the form.
Ensure that all samples are labeled, all labels are completely filled in, and each label is
covered with clear plastic tape. Compare sample label information with the information recorded
on the corresponding field data forms (e.g., the Sample Collection Form) to ensure accuracy.
Make sure that all sample containers are properly sealed.
8.4 Launch Site Cleanup
Load the boat on the trailer and inspect the boat, motor, and trailer for evidence of weeds
and other macrophytes. Clean the boat, motor, and trailer as completely as possible before
leaving the launch site. Follow any state or other requirements associated with nuisance
species, pathogens and/or viruses. Inspect all nets for pieces of macrophytes or other
organisms and remove as much as possible before packing the nets for transport. Pack all
equipment and supplies in the vehicle and trailer for transport. Keep equipment and supplies
organized so they can be inventoried using the equipment and supply checklists presented in
Appendix A. Lastly, be sure to clean up all waste material at the launch site and dispose of or
transport it out of the site if a trash can is not available.
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9.0 FIELD QUALITY CONTROL
Standardized training and data forms provide the foundation to help ensure that data quality
standards for field sampling are met. These Standard Operating Procedures for field sampling
and data collection are the primary guidelines for all cooperators and field teams. In addition,
repeat sampling, and field evaluation and assistance visits will address specific aspects of the
data quality standards for the National Coastal Condition Assessment.
9.1 Repeat Sampling
Repeat sampling will provide data to make variance estimates (for measurement variation
and index period variation) that can be used to evaluate the NCCA design for its potential to
estimate status and detect trends in the target population of sites. The sites identified for repeat
visits are outlined in the site list provided to each state.
A total of 10% of the target sites visited will be revisited during the same field season by the
same field team that initially sampled the site. Repeated samples and measurements are taken
from the same site as the first visit. Each state has a different number of repeat sites; the
number is dependent on the number of base sites the state has and is provided to each state in
the state's site draw. If a site selected for repeat sampling is dropped, then the alternate
assigned to replace it should be revisited. The primary purpose of this "revisit" set of sites is to
collect temporal replicate samples to provide variance estimates for both measurement variation
and index period variation. The revisit will include the full set of indicators and associated
parameters (except fish tissue). We will not be collecting replicate data on fish tissue. Fish
tissue will only be collected on the first visit. The time period between the initial and repeat visit
to a site should be as long as possible, but not less than 2 weeks.
In addition to the normal samples, filter blanks will be collected for Enterococci on both of
the two visits. The teams will filter a small amount (20 ml_) of sterile saline through 4 filters, label
them and write "blank" on the label and field form, and package and submit these samples to
the lab. The filter blanks should be run before the sample is filtered. A detailed description of
the filter blanks is found in table 8-3.
9.2 Field Evaluation And Assistance Visits
A rigorous program of field and laboratory evaluation and assistance visits has been
developed to support the National Aquatic Resource Surveys Program. These evaluation and
assistance visits are explained in detail in the Quality Assurance Project Plan (QAPP) for the
NCCA. The following sections will focus only on the field evaluation and assistance visits.
These visits provide a QA/QC check for the uniform evaluation of the data collection
methods, and an opportunity to conduct procedural reviews as required to minimize data loss
due to improper technique or interpretation of field procedures and guidance. Through uniform
training of field teams and review cycles conducted early in the data collection process,
sampling variability associated with specific implementation or interpretation of the protocols will
be significantly reduced. The field evaluations will be based on the Field Evaluation Plan and
Checklists. This evaluation will be conducted for each unique team collecting and contributing
data under this program (EPA will make a concerted effort to evaluate every team, but will rely
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on the data review and validation process to identify unacceptable data that will not be included
in the final database).
9.2.1 Specifications for QC Assurance
Field evaluation and assistance personnel are trained in the specific data collection methods
detailed in this Field Operations Manual. A plan and checklist for field evaluation and assistance
visits have been developed to detail the methods and procedures. The plan and checklist are
included in the QAPP. Table 9-1 summarizes the plan, the checklist, and corrective action
procedures.
Table 9-1. General Information Noted During Field Evaluation
Field
Evaluation
Plan
Regional Coordinators will arrange the field evaluation visit with each Field Team,
ideally within the first two weeks of sampling.
The Evaluatorwill observe the performance of a team through one complete set of
sampling activities.
If the Team misses or incorrectly performs a procedure, the Evaluatorwill note it on
the checklist and immediately point it out so the mistake can be corrected on the spot.
The Evaluatorwill review the results of the evaluation with the Field Team before
leaving the site, noting positive practices and problems.
Field
Evaluation
Checklist
The Evaluator observes all pre-sampling activities and verifies that equipment is
properly calibrated and in good working order, and NCCA protocols are followed.
The Evaluator checks the sample containers to verify that they are the correct type
and size, and checks the labels to be sure they are correctly and completely filled out.
The Evaluator confirms that the Field Team has followed NCCA protocols for locating
the site.
The Evaluator observes the complete set of sampling activities, confirming that all
protocols are followed.
The Evaluatorwill record responses or concerns, if any, on the Field Evaluation and
Assistance Check List.
Corrective
Action
Procedures
If the Evaluator's findings indicate that the Field Team is not performing the
procedures correctly, safely, or thoroughly, the Evaluator must continue working with
this Field Team until certain of the Team's ability to conduct the sampling properly so
that data quality is not adversely affected.
If the Evaluator finds major deficiencies in the Field Team operations, the Evaluator
must contact a NCCA QA official immediately (e.g., within 24-48 hours) so that
additional correction actions can be taken.
It is anticipated that evaluation and assistance visits will be conducted with each Field Team
early in the sampling and data collection process, and that corrective actions will be conducted
in real time. If the Field Team misses or incorrectly performs a procedure, the Evaluatorwill note
this on the checklist and immediately point this out so the mistake can be corrected on the spot.
The role of the Evaluator is to provide additional training and guidance so that the procedures
are being performed consistent with the Field Operations Manual, all data are recorded
correctly, and paperwork is properly completed at the site.
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9.2.2 Reporting
When the sampling operation has been completed, the Evaluator will review the results of
the evaluation with the Field Team before leaving the site (if practicable), noting positive
practices and problems (i.e., weaknesses [might affect data quality] or deficiencies [would
adversely affect data quality]). The Evaluator will ensure that the Team understands the findings
and will be able to perform the procedures properly in the future. The Evaluator will record
responses or concerns, if any, on the Field Evaluation and Assistance Check List. After the
Evaluator completes the Field Evaluation and Assistance Check List, including a brief summary
of findings, all Field Team members must read and sign off on the evaluation.
If the Evaluator's findings indicate that the Field Team is not performing the procedures
correctly, safely, or thoroughly, the Evaluator must continue working with this Field Team until
certain of the Team's ability to conduct the sampling properly so that data quality is not
adversely affected. If the Evaluator finds major deficiencies in the Field Team operations (e.g.,
major misinterpretation of protocols, equipment or performance problems) the Evaluator must
contact the following QA official:
Joe Hall, EPA National Coastal Condition Assessment Project QA Officer
The QA official will contact the Project Manager to determine the appropriate course of
action. Data records from sampling sites previously visited by this Field Team will be checked to
determine whether any sampling sites must be redone.
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10.0 LITERATURE CITED
American Red Cross. 2006. First Aid/CPR/AED for schools and the community. Third edition.
210 pgs.
Bradley, M.P., Landy, R.B., 2000. The Mid-Atlantic Integrated Assessment (MAIA).
Environmental Monitoring and Assessment 63, 1-13.
Bricker, S.B., Clement, C.G., Pirhalla, D.E., Orlando, S.P., 1999. National Estuarine
Eutrophication Assessment: Effects of Nutrient Enrichment in the Nation's Estuaries.
NOAA, National Ocean Services, Special Projects and the National Centers for Coastal
Ocean Science, Silver Spring, MD, 71 pp.
CENR, 1996. Integrating the Nation's Environmental Monitoring and Research Networks and
Programs: A Proposed Framework. Committee on the Environment and Natural
Resources, White House National Science and Technology Council, Washington, DC.
Chaillou, J.C., Weisberg, S.B., Kutz, F.W., DeMoss, T.E., Mangiaracina, L, Magnien, R., Eskin,
R., Maxted, J., Price, K., Summer, J.K., 1996. Assessment of the Ecological Condition of
the Delaware and Maryland Coastal Bays. EPA/620/R-96/004. US Environmental
Protection Agency, Office of Research and Development, Washington, DC.
Engel, V.D., Summers, J.K., Gaston, G.R., 1994. A Benthic Index of Environmental Condition of
Gulf of Mexico Estuaries. Estuaries 17 (2), 372-284.
Heimbuch, D.G., Wilson, H.T., Robson, D.S., Summers, J.K.., 1995. Design-based Estimation
of the Proportion of Area Degraded and Associated Variance Estimators forEMAP-
Estuaries Sampling in the Louisianian and Virginian Provinces: 1990-1994. Draft report
prepared for US Environmental Protection Agency by Coastal Environmental Services,
Linthicum, MD.
Holland, A.F., 1990. Near Coastal Program Plan for 1990: Estuaries. EPA/600/4-90/33. US
Environmental Protection Agency, Office of Research Development, Narragansett, Rl.
Hunsaker, C., Carpenter, D., 1990. Ecological Indicators for the Environmental Monitoring and
Assessment Program. EPA/600/3-90/060. US Environmental Protection Agency, Office
of Research and Development, Research Triangle Park, NC.
Karr, J.R., Chu, E.W., 1999. Restoring Life in Running Waters, Better Biological Monitoring.
Island Press, Washington, DC.
Klemm, D. J., P. A. Lewis, F. Fulk, and J. M. Lazorchak. 1990. Macroinvertebrate Field and
Laboratory Methods for Evaluating the Biological Integrity of Surface Waters. EPA
600/4-90/030. U.S. Environmental Protection Agency, Cincinnati, Ohio.
Krebs, C.J., 1989. Ecological Methodology. HarperCollins Publishers, New York.
Madden, C. J., K. Goodin, R.J. Allee, G. Cicchetti, C. Moses, M. Finkbeiner, D. Bamford.
Coastal and Marine Ecological Classification Standard. NOAA and NatureServe. 2009.
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page 88
Messer, J.J., Linthurst, R.A., Overton, W.S., 1991. An EPA Program for Monitoring Ecological
Status and Trends. Environmental Monitoring and Assessment 17 (1), 67-78.
National Institute for Occupational Safety and Health. 1981. Occupational Health Guidelines
for Chemical Hazards (Two Volumes). NIOSH/OSHA Publication No. 81-123.
U.S. Government Printing Office, Washington, D.C.
Nelson, J.S., E.J. Grossman, H. Espinosa-Perez, L.T. Findley, C.R. Gilbert, R.N. Lea, and J.D.
Williams. 2004. Common and Scientific Names of Fishes from the United States,
Canada, and Mexico. American Fisheries Society, Special Publication 29, Bethesda,
Maryland.
Occupational Safety & Health Administration (OSHA). 2006. Regulations (Standards - 29 CFR).
Substance technical guidelines for formalin -1910.1048 App A. Occupational Safety &
Health Administration. Washington, DC 20210.
Overton, W.S., White, D., Stevens, D.L., 1991. Design Report of the Environmental Monitoring
and Assessment Program, EPA/600/3-91/053. US Environmental Protection Agency,
Environmental Research Laboratory, Corvallis, OR.
Peck, D. V., Herlihy, AT., Hill, B.H., Hughes, R.M., Kaufmann, P.R., Klemm, D.J., Lazorchak,
J.M., McCormick, F.H., Peterson, S.A., Ringold, P.L, Magee, T., Cappaert, M., 2006.
Environmental Monitoring and Assessment Program-Surface Waters Western Pilot
Study: Field Operations Manual for Wadeable Streams. EPA/620/R-06/003. U.S.
Environmental Protection Agency, Office of Research and Development, Washington,
DC.
Plafkin, J.L, Barbour, M.T., Porter, K.D., Gross, S.K., Hughes, R.M. (1989). "Rapid
bioassessment protocols for use in streams and rivers: Benthic macroinvertebrates and
fish," EPA/440/489/001, U.S. Environmental Protection Agency, Assessment and
Watershed Protection Division, Washington, DC.
Schriver et al. 1995. Impact of Submerged Macrophytes on Fish-Zooplankton- Phytoplankton
Interactions - Large-Scale Enclosure Experiments in a Shallow Eutrophic Lake.
Freshwater Biology 33, no. 2: 255-70.
Summers, J.K., Paul, J.F., Robertson, A., 1995. Monitoring the Ecological Condition of
Estuaries in the United States. Toxicological and Environmental Chemistry 49, 93-108.
U.S. Coast Guard. 1989. Federal Requirements for Recreational Boats. U.S. Department
of Transportation, United States Coast Guard, Washington, D.C. 27 pgs.
U.S. Environmental Protection Agency (USEPA). Research Strategy: Environmental Monitoring
and Assessment. Washington D.C. 2002.
USEPA. 2007. National Rivers and Streams Assessment: Field Operations Manual. EPA-841-
B-07-009. U.S. Environmental Protection Agency, Assessment and Watershed
Protection Division, Washington, DC.
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page 89
USEPA. 2001. National Coastal Assessment: Field Operation Manual. EPA-620-R-01-003.
U.S. Environmental Protection Agency., Office of Research and Development, National
Health and Environmental Effects Research Laboratory.
USEPA. 2000a. EPA Quality Manual for Environmental Programs 5360A1. May 2000.
http://www.epa.gov/quality/qs-docs/5360.pdf
USEPA. 2000b. EPA Order 5360.1 A2 CHG2, Policy and Program Requirements for Mandatory
Agency-wide Quality System, May 5, 2000. http://www.epa.gov/guality/gs-docs/5360-
l.pdf
USEPA. 2001. Methods for Collection, Storage, and Manipulation of Sediments for Chemical
and Toxicological Analyses: Technical Manual. EPA-823-B-01-002. U. S. Environmental
Protection Agency, Office of Water, Washington, D.C.
USEPA (Environmental Protection Agency). 2004. Wadeable Streams Assessment: Field
Operations Manual. EPA 841-B-04-004. U.S. Environmental Protection Agency, Office of
Water and Office of Research and Development, Washington, D.C.
USEPA. 1986. Occupational Health and Safety Manual. Office of Planning and Management
U.S. Environmental Protection Agency, Washington, D.C.
Web Pages:
US EPA Aquatic Monitoring Research: http://www.epa.gov/nheerl/arm
NHD Plus: http://www.horizon-systems.com/nhdplus
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APPENDIX A
List of Equipment and
Supplies
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Page A-2
EQUIPMENT & SUPPLY LISTS
General Equipment
Field Operations Manual and/or laminated
Quick Reference Guide
Covered clipboards
Field forms and sample labels
Clear tape strips for covering labels
Pencils (#2)
Fine-tipped indelible markers
Digital camera with extra memory card &
battery
Maps and access instructions
Sampling permits and/or permission letters
GPS unit with manual and reference card
Batteries
1%-10% Bleach
Calibration cups and standards for multi-
probe unit
Spare parts for multi-probe unit
Electrical and duct tape
Scissors
Plastic storage tub
Cell phone, 2-way radios, and/or walkie-
talkies
Centimeter ruler
Motor
Gas Can
PFDs (1/person)
Type IV PFD (Throwable Life Saving
device)
Bow/Stern lights
Anchor with 75 m line or sufficient to
anchor in 50 m depth
Float to attach to anchor
Sonar Unit
Boat Equipment List
Pingers
First Aid Kit
Extra Boat Plug
Spare Prop Shear Pin
Emergency Tool kit
Hand Bilge pump
Fire Extinguisher
Boat horn
Spare prop
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Sample/Data Collection
Multi-parameter water quality meter with pH,
DO, temperature, and conductivity/salinity
probes (e.g., Hydrolab, YSI, etc.)
20 cm diameter Secchi disk and calibrated
sounding line, marked in 0.5 m intervals
Nitrile gloves
Water sampling bottle (e.g., Niskin) or
sampling pump system
PAR meter with appropriate deck unit and
cables
Thermometer
0.04 m2 Young-modified Van Veen grab
sampler or Standard or Petite Ponar sampler
with plastic tub, drop line, and spare pinch
pin.
Weights and pads for grab
0.5 mm stainless steel sieve; 1.0 mm for CA,
OR, and WA
Sieve box
Plastic tub or bucket for benthic
sediment grab
High-quality stainless mixing pot with lid
Large and small stainless steel spoons
and spatulas for mixing and dispensing
sediment composite
Wde-mouthed funnel
Fine-tipped forceps
Large buckets
Electrical tape
Scrub brush
Squirt bottle
Measuring board (millimeter scale)
Pre-sterilized, 250 mL sample bottle
Sodium thiosulfate tablet
De-ionized water in squirt bottle
Active or passive fish sampling device
(e.g., trawl, seine, hook& line, etc.)
Coolers
Wet ice
Dry ice
Sample Processing/Preservation
Alconox
Aluminum foil squares (3" x 6")
Dl water
100% buffered formalin with Stain
Sterile filtration unit (Nalgene 145/147),
including filter funnel, cap, filter holder, and
receiving chamber
Whatman 47 mm polycarbonate 0.4 micron
filters
Whatman 47 mm 0.7 micron GF/F glass
fiber filters
Sterile disposable forceps
Sterile saline
Wooden bat
Small stainless steel spatula, spoon, or
scoop to transfer sample
Knife or scissors
Plastic cable ties
Sterile filter holder
Hand or electric vacuum pump
Sterile centrifuge tube
60 x 15 disposable Petri dishes sterile
microcentrifuge tubes containing sterile
glass beads
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Sample Storage
250 ml_ amber Nalgene bottle 125 mL Nalgene jar (sediment grain size)
(water chemistry) . 60 mL Nalgene jar (sediment TOC)
2 L amber Nalgene bottle (chlorophyll-a) . 1 ga||on screw-top bucket (sediment
250 mL sterile sample bottle (Enterococci) toxicity)
1 L Nalgene bottles (benthic samples) 50 mL screw-top centrifuge tube
250 mL Nalgene bottle (dissolved Coolers
nutrients) . whirl-Paks
500 mL glass jar (sediment . 2 gallon self-sealing bags (eco fish tissue)
organics/metals) . solvent rinsed aluminum foil, poly tubing
and zip ties (human health fish tissue)
Large plastic composite bags
Packaging/Shipping
Coolers Self-sealing bags
Cooler liners (30 gal garbage bags) Packing/strapping tape
Dry ice (-50 Ibs per site) FedEx airbills
Wet ice (-50 Ibs per site; additional for Class 9 Dangerous Goods label (for dry
shipping) ice shipments)
Sample Collection/Preservation of Additional Great Lakes Indicators
1 L amber Nalgene bottle (phytoplankton) Lugol's solution
Underwater camera system with DVR and 10 mL pipet and pipet bulb
GPS
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A site kit will be provided to the field crews for each sampling site. Site kits will be shipped out
based on the schedule that each field crew provides prior to the start of the sampling season.
Field crew leaders MUST provide a schedule in order to receive the site kits. If your
schedule changes, please report the change as soon as possible to the Site Kit Coordinator
and/or Field Logistics Coordinator. Prior to sampling, inspect each site kit to ensure all supplies
are included.
Supplies provided in each Site Kit:
Field Data Forms
Sample Labels
National Coastal Condition Assessment Fact Sheets
1 250 mL amber Nalgene bottle (water chemistry)
2 1 L Nalgene bottles (benthic samples)
1 500 mL glass jar (sediment organics/metals)
1 60 mL Nalgene jar (sediment TOC)
1 125 mL Nalgene jar (sediment grain size)
11 gallon screw-top bucket (sediment toxicity)
1 250 mL Nalgene bottle (dissolved nutrients)
1 250 mL fecal indicator collection bottle
1 Zip tie
2 50 mL screw-top centrifuge tube (one for measuring enterococci sample for filtering,
one for holding the chlorophyll-a filter)
4 sterile microcentrifuge tubes containing sterile glass beads
Bubble envelope
2 Sterile disposable forceps
Sterile filter holder, Nalgene 145/147
Sterile saline
Large plastic bag (cooler liner)
FedEx airbills for all labs
Dry ice box/label will be included in approximately every 4th site kit
Whirl-Paks
Supplies provided in each Eco Fish Tissue Sampling Kit:
2 gallon self sealing bags
Sandwich size self sealing bags
Large plastic (composite) bags
Plastic cable ties
Tyvek tags with grommets
FedEx airbill for fish tissue lab
Supplies provided in each Human Health Fish Tissue Sampling Kit:
Aluminum foil (solvent-rinsed and baked)
Heavy-duty food grade polyethylene tubing
Large plastic (composite) bags
Plastic cable ties
Tyvek tags with grommets
FedEx airbill for fish tissue lab
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Page A-6
Supplies provided in each Base Kit:
1 2 L amber Nalgene bottle (chlorophyll)
Nitrile gloves
Bottle of 50 sodium thiosulfate tablets
Aluminum foil 3x6"
15" stainless steel spoon
0.5 mm stainless steel sieve bucket; 0.1 mm for CA, OR, WA sampling
Weighted Secchi disk
21 Liter Nalgene wash bottles
13 gallon Rubbermaid Roughneck tote
Graduated cylinder 250 mL
Whatman 47 mm polycarbonate 0.4 u filters
Whatman 47 mm glass fiber GF/F 0.7 u filters
Hand pump
Silicone stopper with filter holder adapter
Spare filter holder adapters
Side-arm filter flask
Disposable petri dishes 60x15
Wde-mouthed funnel
Fine-tipped forceps
Centrifuge tube stand
1 liter of QC check solution (re-order as expiration date approaches)
Tape dispenser
Tape strips
24 ct of 1 Liter Nalgene bottles
Whirl-Paks
Heavy-duty food grade polyethylene tubing and zip ties (for large Eco fish)
12 Spare 2 gallon self sealing bags
Spare sterile saline
Spare 50 mL screw-top centrifuge tubes
Spare sterile microcentrifuge tubes
Spare Sterile filter holder
1 qt Self Sealing Bags (100 count)
Note: sodium thiosulfate tablets, calibration QC check solution, filters, 1 Liter Nalgene bottles,
aluminum foil squares, whirl paks, and disposable nitrile gloves will be provided in the base kit;
you may order more throughout the field season if needed.
Additional Base Kit supplies provided to Great Lakes crews:
Underwater camera system with DVR and GPS
1 liter amber Nalgene bottles (approximately 1 per site on sampling schedule)
500 mL Lugol's solution
10 mL pipette and pipette bulb
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Page B-1
APPENDIX B
Field Forms
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Page B-2
NCCA 2010 SITE VERIFICATION (Front)
Reviewed by (initial):
SITE NAME:
SITE ID: NCCA10- ST~
O
DATE: / f 2 0 1 0 VISIT: O 1 O 2
E OF STATION DEPTH(m): TEAM"
DID YOU SAMPLE THIS SITE?
OYES |f YES, check one below
SAMPLEABLE (Choose method used)
O Marine
O Great Lakes
ARRIVAL TIME: _ : _
DEPART TIME: :
QNO If NO, check one below
NON-SAMPLEABLE-PERMANENT -Replace Site
O Map Error
O Site too shallow for navigation/sampling
O Unsafe
NON-SAMPLEABLE-TEMPORARY-Reschedule
ONo Access
O Temporarily Inaccessible-Fire, etc.
O Other (Explain in comments)
VERIFICATION INFORMATION
Site verified by (fill in all that apply): Q GPS O Local Contact O Signs O Roads QTopo. Map
O Other (Describe Here): O Not Verified (Explain in Comments)
Coordinates Latitude North
TARGET Decimal Degrees
ACTUAL Decimal Degrees
LOCATION
Longitude West satellites X-SITE WITHIN 37M?:
OYES ONO
O <3
liPb Datum Used
Oj4 (e.g. NAD83.WGS84):
HABITAT TYPE: O Tidal River OOpen Water O Marsh/Wetland OEmbayment O Inter-Tidal ORivermouth
O Other, explain:
BOTTOM TYPE: O Coral Reef OOysterBed OGrassBed O Sand O Rocky/Shell QHardpan QMud
O Other, explain:
Debris Present?: | If Yes, TYPE:
OYES ONO ' O Glass O Plastic O Wood
SAV Present?: O Yes ONo ABUNDANCE:
Macroalgae Present?: O Yes ONo ABUNDANCE:
GENERAL COMMENTS:
O Cans O Other, explain:
(Sparse, dense, etc)
(Sparse, dense, etc)
DIRECTIONS TO SITE:
04/22/2010 NCCA Site Verification
8194026369
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NCCA 2010 SITE VERIFICATION (Back)
Reviewed by
(initial):
SITE NAME:
DATE:
2010 VISIT: Q1 O2
SITE ID: NCCA10-
TEAM:
SKETCH MAP - Arrow Indicates North; Mark site L=Launch X=lndex F = Fishing Area
NOTE: If an outline map is attached here, use a continuous strip of clear tape across the top edge.
You can also attach a separate sheet with the outline map on it.
PERSONNEL
NAME
Bio/Chem
Sampling
o
o
o
o
o
Fish
o
o
o
o
o
Forms
Review
O
o
o
o
o
04/22/2010 NCCA Site Verification
1975026369
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NCCA 2010 FIELD MEASUREMENT (Front)
Reviewed by (initial):
SITE ID: NCCA10-
DATE:
/ / 2 0 1 0
CALIBRATION INFORMATION
Instrument manufacturer and model:
Instrument ID number:
Operator:
TEMPERATURE
Thermometer Sensor Reading
Reading ("C) (ฐQ
Flag
Comments
DO
Pressure
(mm Hg)
Calibration
Value
Displayed
Value
Flag
O mg'L
pH
Cal. STD 1 Description
Cal. STD 1 Value Cal. STD 2 Description Cal. STD 2 Value Flag
Cal. STD 1 Description Cal. STD 1 Value Cal. STD 2 Description
CONDUCTIVITY
Cal. STD 2 Value Flag
QUALITY CONTROL CHECK (Perform at least once per week)
TIME:
I
QC BATCH #:
Date Prepared:
COMMENTS:
Parameter TEMP. (ฐC) COND (uS> pH FLAG
No QC Check | standard
performed at
this visit? I Measured
POST-MEASUREMENT CALIBRATION CHECK
pH COND (uS) FLAG
SECCHI DEPTH
DISAPPEARS. REAPPEARS:
Secchi Depth Reading 1:
(m) XX.X:
Reading 2:
Reading 3:
CLEAR TO BOTTOM?
OYes O No
SECCHI FLAG:
Flag Comments
Unique Flag and Comments entered here are for both sides of this Field Measurement form.
Flag codes: K = Sample not collected; U = Suspect sample; F1, F2, etc. = flag assigned by field crew.
04/22/2010 NCCA Field Measurement
9117512028
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v- NCCA 2010 FIELD MEASUREMENT (Back) """""" by """
SITE ID: NCCA10- DATE: / / 2 (
Hydrographic Profile
Intervals (m): 0.1m below surface, 0.5 below the surface, every 1 meter from depths of 1 .0 to '
than 10m. Take the last set of measurements at 0.5m fr
XX.X
NearB
D
O
W
N
C
A
S
T
jttom
U
P
C
A
S
T
DEPTH(m) TEMP. ('C) pM DO|mg/L|
xx.x xx.x xx.xx XX.X
0.1
0.5
SAL (%.) COND (uS)
(Marine) (Great Lakes)
xx.x xxx.x
Om, and every 5 meters thereafter if t
>m the bottom.
1:
LIGHT(AMB) LIGHT(UW)
XXX.X xxxx FLAG
*l>: _
110^
he site is greater
Flag codes: K = Sample not collected; U = Suspect sample; F1, F2, etc. = flag assigned by field crew.
Record any Profile flag and comments on front side of this field measurement form.
04/22/2010 NCCA Field Measurement
49&1512022
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NCCA2010 SAMPLE COLLECTION FORM - (Front) Reviewed by
1 ' (Initials):
SITE ID: NCCA10- DATE: / / 2 0 1 0
WATER CHEMISTRY , CHLOROPHYLL and NUTRIENT COLLECTION (0.5m)
Water Chemistry
(Non-Filtered)
Chlorophyll-a
Nutrients
(Filtered)
Chilled
o
Frozen
O
Chilled
O
Comments No Sample Collected Q
Vฐ' (Fm';)6red Comments No Sample Coltocted Q
Comments No SamPle Collected Q
Use comment section to explain: No measurement, suspect measurement or observation made.
ENTEROCOCCI (Target Volume = 250 mL) No Sample Collected Q
Sample ID
(One unique ID per line)
Filter Blank
OF
Time
Collected
(hhmm)
Depth
Collected
(m)
Sample
Volume
(mL)
Filt. Start
Time
(hhmm)
Volume Filtered
(Target = 50 mL)
Filt. 1
Filt. 2
Filt. 3
Filt. 4
Volume Filtered
(Target = 20 mL)
Filt. 1
Filt. 2
Filt. 3
Filt. 4
Vol.
of
Rinse
Filt. End
Time
(hhmm)
Time
Frozen
(hhmm)
Flag
Flag codes: K = No measurement made, U = Suspect measurement., F1.F2, etc. = flags assigned by each field crew. Explain all flags In comments.
Flag
Comments
GREAT LAKES ONLY
PHYTOPLANKTON (Amber Nalgene 1-L) NO sample collected Q
Sample ID
Preserved
O
Depth
Collected
(m)
Time
Collected
(hhmm)
Time
Preserved
(hhmm)
Comments
U nder water video camera Digital Video Recording NO Sample collected Q
File name Transferred
Format: DVRyymmdd_hhmm_xxx.avi to SD Card Comments
DVR .avi O
04/22/2010 NCCA Sample Collection
8935052620
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page B-7
NCCA 2010 SAMPLE COLLECTION FORM - (Back)
SITE ID: NCCA10-
DATE: f I 2
BENTHIC INFAUNA COLLECTION
0 1 0
No Sample Collected Q
O Van Veen
GRAB AREA : ฐRAB TYPE: 0 Standard Ponar ฐ ฐther:
SIEVE SIZE: O 0-5 mm O 1-0 mm
Depth (cm)
SamDto ID (Must be >7 cml No. O
NOTE:
Jars Preserved Comments
0
SEDIMENT CHARACTERISTICS (Benthic Grab)
COLOR: O Black O Brown O Light Brown O Dark Brown O Gray O Other
SUBSTRATE: O Sand O Muck O Gravel O Cobble O Shellhash O Other
SMELL: O Fishy O Chemical Q Sulphur O None Q Other
SURFACE: O Film O Floe O Nothing Noted O Other
VISIBLE FAUNA: O Yes O No TYPE:
VISIBLE FLORA: O Yes O No TYPE:
SEDIMENT SAMPLE COLLECTION
DISTANCE SEDIMENT COLLECTED:
O Within 37m from X-site O Between 37-100m from X-site O Between 100-500m from X-site (GREAT
LAKES ONLY)
SEDIMENT ORGANICS/METALS (Glass Jar 500 ml)
Sample Volume
Sample ID (Target = 250 mL) Chi
C
ted Comments
)
No Sample Collected Q
SEDIMENT GRAIN SIZE (Nalgene 125ml)
Sample Volume
Sample ID (Target = 100 mL) Chi
C
Sample Volume
Sample ID (Target = 50 mU Chi
C
led Comments
)
No Sample Collected Q
SEDIMENT TOC (Nalgene 60ml)
led Comments
)
No Sample Collected Q
SEDIMENT TOXICITY (1 gal Screw Top Bucket) NO sample collected Q
Sample ID
Sample Volume
(Taraet = 3D
Cnllled
O
Comments
Use comment section to explain: No measurement, suspect measurement or observation made.
04K2/20W NCCA Sample Collection
3003052621
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page B-8
NCCA2010 ECO FISH COLLECTION (Front)
Reviewed by (initial):
SITE ID: NCCA10-
DATE:
/ 2 0 1 0
Collection Method
O TRAWL
O GILL NET
O OTHER EXPLAIN:
O HOOK & LINE OSElNE
O PURCHASED DOCKSIDE
Trawl/Seine Info: HELMSMAN:
LINE OUT (m):
Trawl/Seine Start:
Decimal Degrees
HEADING IN DEGREES
MAGNETIC:
LONGITUDE:
START TIME:
Trawl/Seine End:
LATITUDE:
Decimal Degrees
LONGITUDE:
If Seine: LENGTH:
If Gill Net: LENGTH:
(m) START TIME:
Flag Codes: K - no measurement made; U - suspect measurement; F1, F2, etc - nags assigned by each field crew Explain all flags in comments section.
Flag
04/22/2010 NCCA ECO Fish Collection (Front)
050S346545
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page B-9
NCCA2010 ECO FISH COLLECTION (Back)
Reviewed by (initial):
SITE ID: NCCA10- DATE: / / 2 0 1 0 PAGE: OF
FISH TISSUE SAMPLE O NO SAMPLE COLLECTED
FISH ALL WITHIN 75% OF LARGEST SPECIMEN Q
Genus Species Total Length (mm) Frozen Comments
.01
.02
.03
.04
.05
.06
.07
.08
.09
.10
.11
.12
.13
.14
.15
.16
.17
.18
.19
.20
O
O
O
O
O
O
O
O
O
O
O
O
O
O
O
O
O
O
O
O
The eco fish composite must consist of at least 5 fish of adequate size to provide a total weight of 500 grams of whole-body tissue.
9233044667
04/22/2010 NCCA ECO Fish Collection (Back)
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page B-10
NCCA2010 HUMAN HEALTH FISH COLLECTION (Front)
Reviewed by (initial):
SITE ID: NCCAGL10-
DATE:
/ 2 0 1 0
Collection Method
O TRAWL
O GILL NET
O OTHER EXPLAIN:
O HOOK & LINE
SEINE
Trawl/Seine Info: HELMSMAN:
LINE OUT (m):
Trawl/Seine Start:
Decimal Degrees
HEADING IN DEGREES
MAGNETIC:
LONGITUDE:
START TIME:
Trawl/Seine End:
LATITUDE:
Decimal Degrees
LONGITUDE:
If Seine: LENGTH:
If Gill Net: LENGTH:
(m) START TIME:
Flag Codes: K - no measurement made; U - suspect measurement; F1, F2, etc - nags assigned by each field crew Explain all flags in comments section.
Flag
04/22/2010 NCCA Human Health Fish Collection (Front)
5721053452
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
PageB-11
NCCA2010 HUMAN HEALTH FISH COLLECTION (Back) R..I
SITE ID
NCCAGL10- DATE: / / 2 0 1 0 PAGE: OF
FISH TISSUE SAMPLE O NO SAMPLE COLLECTED
SAMPLE ID
FISH ALL WITHIN 75% OF LARGEST SPECIMEN Q
Genus Species Total Length (mm) Frozen Comments
.01
.02
.03
.04
.05
1
1
O
O
O
O
O
O
O
O
O
O
Human health fish composites should consist of 5 similarly-sized adult fish of the same species that will collectively yield about 500 g of fillet tissue
(refer to Frequently Asked Questions for possible exceptions).
7461152602
04/22/2010 NCCA Human Health Fish Collection (Back)
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page B-12
NCCA 2010 SITE ASSESSMENT (Front)
Reviewed by (initial):
SITE ID: NCCA10-
DATE:
2010
SHORELINE ACTIVITIES AND DISTURBANCES OBSERVED
(Intensity: Blank=Not observed, L=Low, M-Moderate. H=Heavy)
Residential
Recreational
Agricultural
Industrial
Management
M H Residences
L M H Hiking Trails
H Maintained Lawns
H Construction
M H Pipes. Drains
M H Dumping
M H Rom.
M H Bridge/Culverts
M H S.wig. Trealmen
H Parks. Campgrounds
H Primitive Parks, Camping
H Trash/Litter
H Surface Films
H Dunes
H Beach
L M H Cropland
L M H Pasture
L M H Livestock Use
L M H Orchard.
L M H Poultry
L M H Irrigation Equip.
L M H Water-Withdrawal
M H Industrial Plants
H Mines/Quarries
H Oil/Gas Wells
H Power Plants
H Logging
H Evidence of Fin
H Odors
L M H Chemica! Treatment
L M H Angling Pressure
L M H Dredging
L M H Channelization
L M H Water Level Fluctuation!
L M H Shoreline Hardening
L M H Dredge Material
SITE CHARACTERISTICS (200 m radius)
Waterbody
Character
Pristine
Appealing
O5
05
O4
04
O3
03
02
02
O1
01
Highly Disturbed
Unappealing
Dominant
Land Use
Dominant Land Use _
Shoreline O Forest
rf Forest, Dominant Age
Class
O 0 - 25 yrs.
O Agriculture O Range
O 25 - 75 yrs. O * 75 yr
O Urban
O Suburban/Town
WEATHER
GENERAL ASSESSMENT (Biotic integrity, Vegetation diversity, Local anecdotal information)
04/22/2010 NCCA Site Assessment
7216195652
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Field Operations Manual Date: April 23, 2010
Page B-13
NCCA 2010 SITE ASSESSMENT (Back) """"""""""'""'-
SITE ID: NCCA10- DATE: i i 2 0 1 0
1
GENERAL ASSESSMENT (continued)
04/22/2010 MCCA Site Assessment 0854195653
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page C-1
APPENDIX C
Example of Great Lakes
Disinfection Protocols
from Wisconsin DNR
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page C-2
Boat and Gear Disinfection Protocol
Boat and trailer cleaning guidelines to prevent the spread of aquatic invasive species have been
widely distributed to the public through a variety of publications, pamphlets, signs, etc. The
guidelines consist of a nationally-accepted set of prevention steps. While disinfection is not a
required prevention step for the general public, some boaters may be interested in the
disinfection procedures followed by the Wl DNR. Please note: the first three steps (Inspect and
Remove, Drain, and Dispose) listed below are required.
The following steps shall be taken every time a boat, equipment or gear is moved
between waters to avoid transporting invasive species and/or pathogens:
1. Inspect and remove aquatic plants, animals, and mud from your boat, trailer, equipment
and gear.
2. Drain all water from your boat, motor, live well, bilge, transom wells, as well as from your
equipment and gear, including but not limited to tracked vehicles, barges, silt or turbidity
curtain, hoses, sheet pile and pumps.
3. Dispose of unwanted aquatic plants and animals in an appropriate way.
4. Disinfect your boat, equipment and gear by either:
Washing with -212ฐ F water (steam clean), OR
Drying thoroughly for 5 days after cleaning with soap and water and/or high
pressure water, OR
Disinfecting with either 200 ppm (0.5 oz per gallon or 1 Tablespoon per
gallon) Chlorine for 10 minute contact time or 1:100 solution (38 grams per
gallon) of Virkon Aquatic for 20 to 30 minute contact time. Note: Virkon is not
registered to kill zebra mussel veligers nor invertebrates like spiny water flea.
Therefore this disinfect should be used in conjunction with a hot water (>104ฐ
F) application.
Safety Precautions for Disinfectant Use
Virkon-A:
1. Receive and be required to read a copy of the Virkon-A Materials Safety Data Sheet
(MSDS) for the product.
2. Wear chemical splash goggles.
3. Wear a face shield where the possibility exists for face contact due to splashing or
spraying of the material.
4. Wear impervious clothing to prevent contact with skin, (gloves, pants, jacket, hood, and
boots) or a Tyvek style full body suit.
In addition, all employees who handle or mix Virkon-A in powder form and prefer to wear
a dust mask respirator when handling powder, may do so in compliance with the DNR
Respiratory Protection Program Handbook MC 9180.5 Voluntary Use requirements.
Bleach:
Follow precautions 2, 3, and 4 (above).
o Chlorine Wear eye protection, rain gear, gloves if spraying. Stay upwind of the
spray. Will break down in sunlight and when in contact with organic material. Is
corrosive to metal and rubber. Is toxic to fish at these concentrations so rinse
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page C-3
well after disinfection or neutralize with sodium thiosulfate. For neutralizing
chlorine, spray sodium thiosulfate in an 800 ppm solution (3 grams per gallon of
water) on all surfaces after the disinfection period is over. Rinse with water from
the next lake to remove any remaining sodium thiosulfate.
o Virkon Aquatic This is a disinfectant in the peroxygen (hydrogen peroxide) family. It
is a powder. It is 99.9% biodegradable and breaks down to water and oxygen
and is not corrosive at the working dilution. Wear dust mask if mixing powder and
eye protection, rain gear and gloves if spraying. Stay upwind of spray.
Sources of disinfectants
Chlorine - Household bleach (5.25% chlorine) can be purchased from a grocery or convenience
store. HTH is granular chlorine (70% calcium hypochlorite) and can be purchased from a pool
supply company.
Sodium Thiosulfate - Commonly used to neutralize chlorine and iodine. It should be available
at a pool supply company or from a chemical supply company.
Virkon Aquatic is available from Western Chemical. It is the same formulation, but without the
perfume and dye, and the label addresses specific fish pathogens. Their phone is 1-800-283-
5292.
Disinfection measures must be taken prior to moving boats, equipment and other gear from one
waterbody to another. They are not needed daily when sampling the same waterbody or for law
enforcement equipment in emergency situations. In cases where boats and gear return to state
hatcheries, disinfection should be done in a location away from ponds and water supplies to
prevent disinfectant or untreated water from entering those areas. Every effort should be made
to keep the disinfection solution and rinse water out of surface waters.
To the extent practicable, equipment and gear used on waters known to be infested with
invasive species and viruses should not be used on other non-infested waters. The following are
some helpful hints to consider when planning your work in water.
^Organize your sampling so the work in infested waters is always done last.
Dlf a high percentage of your work is done in waters with invasive species, consider
dedicating certain gear to be used only in those waters.
D Depending on the type of work you are doing, it may be possible to work with lake
volunteers and use their boats to collect samples. That way only your gear needs to be
disinfected.
The following methods are provided to assist staff when disinfecting equipment and gear
commonly used by department staff.
Nets
Organic debris should be removed prior to disinfection. Power washing is not required, but nets
could be sprayed with a garden hose to remove debris. Nets may be steam cleaned, washed
and dried thoroughly for five days or treated with a disinfection solution. Nets should be placed
-------
National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page C-4
in the disinfection solution for the appropriate contact time for the solution being used. After
rinsing, the nets can be used immediately, or hung to dry.
Personal protective gear, including rain gear, gloves, boots/waders
Scrub personal protective gear with the disinfection solution. After scrubbing, the gear should be
kept wet with the disinfection solution for the appropriate contact time. Rinse with clean water or
water from the next waterbody. Alternatively, personal gear may be steam cleaned or dried
thoroughly for five days after cleaning with soap and water.
Dip nets, measuring boards and other sampling gear
Remove any organic material from sampling gear. There are several options for disinfecting
smaller gear. Dissolved oxygen probes and other sensitive electronic sampling gear may be
damaged by disinfection solution and should only be rinsed with clean water. For other gear
used in water choose one of the following options:
Option one: The gear can be sprayed with the disinfection solution and a wet surface
maintained for the appropriate contact time. The gear should be rinsed with clean water
or water from the next waterbody before it is used again.
Option two: Fill a tub with disinfection solution and place all equipment in the tub for the
appropriate contact time. The gear should be rinsed with clean water or water from the
next waterbody before it is used again.
Option three: Use a completely new set of gear for each waterbody during the work day
and disinfect all gear at the end of the day using option one or two.
Boats, trailers, and live wells
Remove organic material from boats, trailers, and live wells. Drain water from live wells, bilges
and pumps. The outside and inside of the boat, trailer, live wells, bilges, and pumps should be
sprayed with the disinfection solution and left wet for the appropriate contact time. The inside of
the live wells, bilges and pumps should be made to contact the solution for the appropriate
contact time as well. Run pumps so they take in the disinfection solution and make sure that the
solution comes in contact with all parts of the pump and hose. The boat, trailer, bilges, live well,
and pumps should be rinsed with clean water or water from the next waterbody after the
appropriate contact time. Every effort should be make to keep the disinfection solution and rinse
water out of surface waters. Pull the boat and trailer off the ramp and onto a fairly level area and
away from street drains to minimize potential runoff into surface waters.
Motors
After removing from the water, tip the motor to the down position and start the motor for several
seconds or turn motor over several times to dispel water from the cooling system. Alternatively
and especially for motors moored in water for several days or more, emerge the lower unit in a
bucket of disinfectant and run the motor to ensure contact with all internal parts and allow for the
appropriate contact time. Or, rig up a short (6 foot) piece of garden hose to lower unit muffs. A
pail of the disinfectant can be set in the back of the boat and gravity fed to the lower unit to run
the disinfectant through the motor. Allow solution to remain in motor for the appropriate contact
time. The hose will need to be primed to start the gravity flow because the lower unit does not
create enough suction to prime the hose. A non-corrosive (Virkon Aquatic) is recommended for
use to protect the impeller. Rinse with clean water or water from the next waterbody.
Heavy Equipment
For heavy equipment steam-cleaning is an effective method of disinfection.
-------
National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page D-1
APPENDIX D
Shipping and Tracking
Guidelines
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page D-2
Tracking Forms
If you have access to a computer, fill out the electronic tracking forms:
Be careful to fill out all information accurately and completely.
If you do not have a printer, you will need to fill out and include the scannable form in the
shipping cooler. This is true for all tracking forms listed below.
4 Tracking Forms
1 - Tracking and Sample Status - WRS
This form is filled out for the samples that are shipped immediately after each sampling
event (water chemistry, chlorophyll-a, sediment grain size, sediment TOC, and the
dissolved nutrients samples).
All of these samples will be sent together in one cooler to the EPA Corvallis lab.
Save form according to the file naming convention on the bottom of form.
Email to address on bottom of form and print form to include in the shipping cooler.
*Emailing the electronic WRS form serves as the "status report" for that sampling event.
2 - Tracking (Batched Samples)
BATCHED samples are held & shipped within 2 weeks of collection. Send form when
SHIPPED.
Use one tracking form for each laboratory.
Save form according to the file naming convention on the bottom of form.
Email to address on bottom of form and print form to include in the shipping cooler.
3 - Tracking - Fish Tissue
Fish for ecological tissue analyses (eco fish) will be collected at all sites.
A separate tracking form is provided for eco fish.
The eco fish will be sent to the eco fish tissue lab.
Save form according to the file naming convention on the bottom of form.
Email to address on bottom of form and print form to include in the shipping cooler.
4 - Tracking - Human Health Fish Tissue
A subset of 150 Great Lakes sites will be sampled for human health contaminants in fish
tissue.
A separate tracking form is provided for human health fish.
The human health fish will be sent to the human health fish tissue lab.
Save form according to the file naming convention on the bottom of form.
Email to address on bottom of form and print form to include in the shipping cooler.
-------
National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page D-3
If you cannot use a computer before shipping:
Fill out the paper version of the tracking form.
Notify the Information Management Center (contact info on bottom of form) - either FAX
form or leave voice message with ALL info from the form.
Include the form in the shipping cooler.
Make sure to FAX or leave a voice message BEFORE the form is sealed in the cooler!
Status Report
After each site, the Field Team Leader must file a status report with the Information
Management Center and the Field Logistics Coordinator to track visits/samples and to
describe activities, problems, and requests.
Emailing the electronic WRS form serves as the status report and will go to both the
Information Management Center and the Field Logistics Coordinator.
If the form cannot be emailed, faxing or phoning the information serves as the status
report.
SHIPPING GUIDELINES
Before shipping, it is very important to preserve each sample as directed in the sample
collection portion of this Field Operations Manual.
Preserve the samples as specified for each indicator before shipping (Figure D-1).
Be aware of the holding times for each type of sample (Table D-1):
Water chemistry, dissolved nutrients, sediment grain size and sediment TOC samples
must be shipped within 24 hours of collection.
Chlorophyll-a samples have a longer holding time, but will be sent with the water
chemistry samples since they are analyzed by the same laboratory.
The benthos samples must be preserved immediately upon collection; they may then be
sent in batches to the appropriate laboratory.
The sediment toxicity and sediment chemistry (organics/metals) samples have a two
week holding time. These two sample types will be shipped to the same sediment lab,
but no more than two visits worth of samples will be able to fit in a single cooler. The
extra space within the cooler will allow for sufficient wet ice for shipping. Securely tape
the cooler drainage open to prevent pressure build-up in the cooler.
Secure the cooler with strapping tape.
Enterococci samples must be filtered and frozen on dry ice within 6 hours of collection.
They can be batched and sent every two weeks.
Fish tissue samples must be frozen on dry ice as soon as possible (hold on wet ice until
freezing on dry ice).
See "Dry Ice Shipping Protocols" at the end of this Appendix.
-------
National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page D-4
Figure D-1. Sample Packaging and Shipping Flow Chart.
WATER ^
CHEMISTRY
(CHEM)
250 ml
amber bottle^
WATER ^
CHLOROPHYLL
(CHLA)
Filter in 50 ml
I tube )
1
1
'"DISSOLVED"^ f SEDIEMNT^ f SEDIMENT^
NUTRIENTS GRAIN SIZE TOC
(NUTS) (SEDG) (SEDC)
250 ml 125 ml 60 ml
bottle J \^ bottle j \ bottle ^
r ^
r ECO FISH ^
TISSUE
(FTIS)
double bag'd
V J
' V \' \
Hold on wet ice
r
Tape lid
;
Preserve
on wet ice
.
ฑ
Prepare 1
Filter
ฑ
Tape lid,
wrap in foil,
Place in
whirl-pak
J
Freeze on
dry ice
\
Tape lids
T
r ENTERO- ^
COCCI
(ENTE)
4 filters in
^ via s ^
1
Hold in live
well
1
Hold on
wet ice
r ^
ID, Measure,
and Dispatch
T
TOXICITY
(SEDX)
1 gal bucket
^ J
\
;
SEDIMENT
ORGANICS/
METALS
(SEDO)
500 ml glass
Hold on wet ice
' i
Prepare 4
filters
r i
Plastic bag
(Double)
Preserve on wet ice
' i
r
Mix and place
~3L into 1 gal
bucket
' T
Place in
bubble wrap
bag
.
Freeze on
dry ice
,
SHIP ON WET ICE AS SOON AS POSSIBLE AFTER
Y i
COLLECTION
' i
r
Hammer
lid
' 1
Freeze on
dry ice
.
SHIP ON
DRY ICE
(May be
batched)
,
OVERNIGHT COURIER REQUIRED
Saturday delivery OK
J
\^
i
T 1
I
WRS - EPA Lab """--x.
Corvallis, OR ^
r
1
r
Mix and place
250 ml into
500 ml bottle
r BENTHOS ^
(BENT)
l-LBottle(s)
1
Sieve
sample in
field
^
'
Composite into
l-Lbottle(s),
< 1/2 full
1
Tape lid
i
r
Store refrigerated
' 1
Ship in
batches
within 2
weeks
.
OVER-
NIGHT
COURIER
NO
Saturday
delivery!
r
OVER-
NIGHT
COURIER
NO
Saturday
delivery!
r i
r
Add 100mL
buffered
formalin, fill
with water
Tape lid(s)
' 1
SHIP ON WET ICE
Together in batches
after 2 v sits
(Do not hold more than 2 weeks)
,
r
^
Great Lakes Only
HUMAN
HEALTH
FISH TISSUE
(HTIS)
Foil, poly
tube, & bag'cL
^
r
Hold in live
well
;
PHYTO- ^
PLANKTON
(PHYT)
1-L amber
^ Bottle j
\
r
Hold on
wet ice
ID, Measure,
and Dispatch
;
;
Add 10 ml
Lugol's
within 2 hrs
Foil wrap,
poly tube,
plast c bag
T
;
Tape lid
' i
Freeze on
dry ice
' 1
Ship in
batches
within 2
weeks
j 1
OVERNIGHT COURIER
NO
Saturday delivery!
/FTIS\ /NERL\ S
( Lab )( REPA (
V 1 \ Region / V
L .i
GLEC -or- \ I
Tetra Tech ) [
(See Below) J \
r
OVER-
NIGHT
COURIER
NO
Saturday
delivery!
i
r
' BENT >
Lab
V J
r
Store
refrigerated
' i
SHIP ON
DRY ICE
(May be
batched)
I
r
SHIP ON
WET ICE
(May be
batched)
r i
OVER-
NIGHT
COURIER
NO
Saturday
delivery!
UNDER
WATER
VIDEO
(UVID)
Files on SD
Card j
\
r
Save files
to SD card.
Backup
files to
computer
daily.
;
>
Send SD
card at end
of field
season.
'
r
Ship in
padded
envelope
r i
OVER-
NIGHT
COURIER
NO
Saturday
delivery!
r
Regular
ground
shipment
OK
/HTIS\ /MED -\ /MED A
( Lab 1 1 EPA EPA
V yV Lab yV Lab y
Field Forms (PACK): All field forms should be reviewed and sent in to the Information Management Coordinator (WED - Corvallis) every 2 weeks
Sediment Toxicity (SEDX) and Sediment Organics/Metals (SEDO) will be shipped together to either Tetra Tech or GLEC based on the state in which the
sampling took place. Refer to the note enclosed with the FedEx airbills to determine the correct destination lab.
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page D-5
WATER CHEMISTRY, CHLOROPHYLL-a and DISSOLVED NUTRIENTS
Water Chemistry
Stored in a 250ml_ amber Nalgene bottle
Confirm that the labels with sample IDs are completed and covered with clear tape.
Seal the lid with plastic (electrical) tape.
Place the bottle in a 1 qt self-sealing plastic bag and place inside the cooler liner.
Chlorophyll-a
Filter stored in a 50 ml_ screw-top centrifuge tube wrapped with aluminum foil
Confirm that the labels with sample IDs are completed and covered with clear tape.
Seal the lid with plastic (electrical) tape.
Cover the tube with aluminum foil.
Place the centrifuge tube in a whirl-pak.
Place the whirl-pak in a small (sandwich size) self-sealing plastic bag and place
inside cooler liner with water chemistry sample.
Dissolved Nutrients Sample
Filtrate from chlorophyll-a filtration collected in a 250 ml_ Nalgene bottle.
Confirm that the labels with sample IDs are completed and covered with clear tape.
Seal the lid with plastic (electrical) tape.
Place the bottle in a 1 qt self-sealing plastic bag and place inside cooler liner with
water chemistry sample..
SEDIMENT GRAIN SIZE AND TOC SAMPLES
Stored in 125 ml_ bottles (grain size) and 60 ml_ bottles (TOC).
Confirm that the labels with sample ID is completed and covered with clear tape.
Seal the lids with plastic (electrical) tape.
Place each of the bottles in separate small (sandwich size) self-sealing plastic bags.
Place the bags in a 1 gal self-sealing plastic bag and place inside cooler liner with water
chemistry sample.
SEDIMENT TOXICITY AND ORGANICS/METALS SAMPLES
Stored in 1 gallon screw-top bucket (toxicity) and 500 ml_ glass jar (organics/metals).
Confirm that the labels with sample ID is completed and covered with clear tape.
Seal the lids of glass jars with plastic (electrical) tape.
Hammer the lids of plastic buckets in clockwise direction to close securely
Wrap each of the 500 ml_ glass jar in bubble wrap and place in separate 1 qt self-sealing
plastic bags.
Place the bags in a 1 gal self-sealing plastic bag and place inside cooler liner with
sediment toxicity samples
These two sample types will go to the same sediment lab, but no more than two visits
worth of samples (2 buckets and 2 glass jars) will be able to fit in a single cooler. This is
to allow for enough space for wet ice in the cooler.
Do not hold these samples longer than 2 weeks.
UNDERWATER VIDEO RECORDING FILES (GREAT LAKES SITES ONLY)
One minute of good quality video is recorded on the system DVR at the sampling site.
Transfer the files to the SD card provided daily.
Backup the video file daily or as often as possible to a computer hard drive.
Send SD card to MED lab in Duluth, MN at end of field season.
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page D-6
PHYTOPLANKTON (GREAT LAKES SITES ONLY)
Stored in a 1 L amber Nalgene bottle
Confirm that the labels with sample IDs are completed and covered with clear tape.
Add 10 mL Lugol's solution with 2 hours of sample collection
Seal the lid with plastic (electrical) tape.
Place the bottle in a 1 gal self-sealing plastic bag and place inside a cooler with liner.
Shipping with wet ice is preferred, but not required for these samples.
Samples can be held for up to 2 weeks and shipped in batches to the laboratory for
analysis.
BENTHIC INVERTEBRATE SAMPLES
Preserved in 100 % buffered formalin and sealed at the site with plastic (electrical) tape.
Confirm that the label with sample ID is completed and covered with clear tape.
Check to make sure jars are sealed with electrical tape.
Place up to ten 1 L jars in each cooler.
Surround the jars with crumpled newspaper, vermiculite, or other absorbent material.
Samples can be held for up to 2 weeks and shipped in batches to the laboratory for
analysis.
FISH TISSUE SAMPLES
The samples need to be frozen as soon as possible after collection (within 6 hours).
Pack the cooler with 50 Ibs of dry ice.
Refer to the DRY ICE SHIPPING PROTOCOLS at the end of this Appendix.
Samples may be stored on dry ice for a maximum of 24 hours. Sampling teams have the
option, depending on site logistics, of:
shipping the samples packed on dry ice (50 pounds, layered to ensure direct contact
between fish and dry ice), via priority overnight delivery so that they arrive at the
sample preparation laboratory within 24 hours of sample collection, or
freezing the samples within 24 hours of collection at <-20ฐC, and storing the frozen
samples until shipment within 2 weeks of sample collection (frozen samples will be
packed on layered dry ice and shipped to the sample preparation laboratory via
priority overnight delivery service).
ENTEROCOCCI SAMPLES
The sample needs to be filtered and frozen as soon as possible after collection (within 6 hours).
4 filters are placed in separate microcentrifuge tubes with ceramic beads
Confirm that the tubes are properly sealed and labeled with the volume of sample filtered
(do not cover the small labels on the microcentrifuge tubes with tape).
Place the 4 microcentrifuge tubes in the bubble wrap envelope.
Confirm that the bubble wrap envelope is labeled with the appropriate sample ID and
volume of sample filtered. Covered outer label with clear plastic tape.
Place the bubble wrap envelope in the cooler and close.
Pack the cooler with 10-15 Ibs of dry ice (10 Ibs if using dry ice blocks or slices, 15 Ibs if
using dry ice pellets).
Refer to the DRY ICE SHIPPING PROTOCOLS at the end of this Appendix.
Samples can be held frozen and shipped in batches to the laboratory for analysis.
Do not hold these samples longer than 2 weeks.
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page D-7
DRY ICE SHIPPING PROTOCOLS
1. Indicate dry ice on shipping airbill
Fill out Section 1 and Section 3 of the Fed Ex airbill with your Sender and
Recipient address and phone number.
In Section 4, check "FedEx Priority Overnight."
In Section 5, check "Other."
In Section 6, under "Does this shipment contain dangerous goods?":
Check "Yes/Shipper's Declaration not required."
Check "Dry Ice," and fill out" 1 x (ami, of dry ice in kg) kg"
In Section 7, fill out weight and declared value of package.
2. Label cooler with a Class 9 Dangerous Goods label (available from FedEx) (Fig. D-2).
Shipper's Declaration not Required
Part E is required
Dry Ice amount must be in
kilograms.
Note: 2 Ibs.= 1 kc
^^^^iAiaybills/aJrtiills must have the following:
^^ * 1. "Dangerous Goods Shipped
Declarators not Required'1.
2. Dry Ice; 9; UN 1815; 111
, 3. * Kg 901
w
Place the label on the front
side of the cooler, not the
top of the cooler.
Fill out #3 in the top right
hand corner of the label
with the same information
as in Section 6 of the
FedEx airbill.
Declare the weight of the
dry ice again in the lower
left hand corner.
Fill out the Sender
("Shipper") and Recipient
("Consignee") address on
the bottom of the label.
Figure D-2. Class 9 Dangerous Goods label.
3. Securely tape the cooler drainage open to prevent pressure build-up in the cooler. This
is critical to ensure proper venting of the dry ice.
4. Secure the cooler with strapping tape.
5. Place the completed airbill on the top of the cooler.
NOTE: Not all FedEx locations will accept shipments containing dry ice. Dry ice shipments can
be shipped from "FedEx staffed" locations. You can also arrange for a pick-up from your lab or
hotel. Dry ice shipments usually cannot be shipped from FedEx Kinko's Office and Print
Centersฎ or FedEx Authorized ShipCenterฎ locations. These types of locations are
differentiated on FedEx.com in the "Find FedEx Locations" feature. Please be sure to call in
advance to ensure your location will accept the package for shipment.
TRACKING FORMS
A Tracking Form must be filled out to accompany each sample shipment. Please refer to
Figures 3-2 through 3-5 for examples of Tracking Forms completed for both unpreserved and
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National Coastal Condition Assessment
Field Operations Manual Date: April 23, 2010
Page D-8
preserved samples. Be very careful to fill in the information correctly and legibly, especially the
airbill number, Site ID, and Sample ID numbers. Use the codes on the bottom of the form to
indicate sample type. Fill out a separate tracking form for each destination laboratory.
The Tracking Form is to be placed in a self-sealing plastic bag and included inside the shipping
container. Before sealing the container, remember to submit the status report (via email) to
sampletracking@epa.gov (see Section 3.2.5); you will need the information on the tracking form
to fill out the status report form. For preserved samples, submit a tracking form both when the
samples are brought to the holding facility AND when they are shipped to the appropriate
laboratory. For each shipment, you must print the electronic form or fill out a scannable tracking
form to include in the cooler and submit the electronic status report.
When ice is used for shipment (water chemistry, dissolved nutrients, chlorophyll-a, sediment
grain size and TOC):
Ensure that the ice is fresh before shipment; pack the entire cooler full with ice.
Line the cooler with a large, 30 gallon plastic bag.
Contain the ice separately within numerous 1 gallon self-sealing plastic bags.
Double-bag the ice.
Use white or clear bags and label with a dark indelible marker. Label all bags of ice
as "ICE" to prevent misidentification by couriers of any water leakage as a possible
hazardous material spill.
Place bagged samples and bags of ice inside the cooler liner and seal the liner.
Secure the cooler with strapping tape.
When dry ice is used for shipping (fecal indicator and fish tissue):
Indicate dry ice on shipping airbill.
Label cooler with a Class 9 Dangerous Goods label.
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National Coastal Condition Assessment
Field Operations Manual
Date: April 23, 2010
Page D-9
Table D-1 Sample Packaging and Shipping Summary
SAMPLE TYPE
Water Chemistry
Chlorophyll-a
Collection
Processing
Dissolved Nutrients
Sediment - Organics/Metals
Sediment- Grain size
Sediment - TOC
Sediment - Toxicity
Benthic macroinvertebrates
Enterococci
Collection
Processing
Filter Blanks
(Revisit sites)
Eco Fish Tissue
Phtyoplankton (Great Lakes Only)
Underwater Video (Great Lakes Only)
Human Health Fish Tissue
(Subset of Great Lakes sites)
SAMPLE
TARGET
VOLUME
250 mL
2L
Readily visible
stain in filter -
max of 2000
mL filtration
250 mL of
filtrate from chl
a filtering
250 mL
100mL
50 mL
3L
All organisms
in grab(s)
250 mL
4 - 50 mL
filtrations
4-20mL
filtrations of
sterile saline
5 - 20+ fish
(500 g whole-
body tissue)
1 L
1 minute video
5 Fish
(500 g of fillet
tissue)
CONTAINER
250 mL amber Nalgene
bottle
2L amber Nalgene bottle
Filter in 50 mL centrifuge
tube
250 mL Nalgene bottle
500 mL glass jar
125 mL Nalgene bottle
60 mL Nalgene
1 gallon screw top bucket
1 L Nalgene bottle(s)
Pre-sterilized 250 mL
Nalgene bottle
4 filters in microcentrifuge
tubes
4 filters in microcentrifuge
tubes
2 gallon self-sealing bag(s)
Large outer plastic bag
1 L amber Nalgene bottle
Save to DVR
Wrapped individually in
solvent rinsed foil
Sealed in poly tubing
Large outer plastic bag
PRESERVATIVE
Wet ice in field
Wet ice in field
Dry ice in field after filtration
Wet ice in field
Wet ice in field; refrigerate to hold
Wet ice in field
Wet ice in field
Wet ice in field; refrigerate to hold
100 mL 100% buffered formalin,
fill to rim with water
Wet ice in field
Dry ice in field; hold in freezer;
MUST be filtered & frozen within 6
hours of collection
Dry ice in field; hold in freezer
Dry ice in field; hold in freezer
10 mL Lugols solution within 2 hrs
Wet ice in field; refrigerate to hold
Save files to SD card daily
Backup to computer often
Dry ice in field; hold in freezer
SHIPPING TIME FRAME
Immediate
Immediate
mmediate
Batch up to 2 weeks
Immediate
mmediate
Batch up to 2 weeks
Batch up to 2 weeks
Batch up to 2 weeks
Batch up to 2 weeks,
send with regular ENTE
sample from site
Batch up to 2 weeks
Batch up to 2 weeks
Ship SD card at end of
field season
Batch up to 2 weeks
PACKAGING FOR
SHIPMENT
Ship in cooler with wet ice
Ship in cooler with wet ice
Ship in cooler with wet ice
Ship in cooler with wet ice
Ship in cooler with wet ice
Ship in cooler with wet ice
Ship in cooler with wet ice
Ship in cooler or sturdy
container
Ship in cardboard cooler
box (provided)
with DRY ICE
Ship in cardboard cooler
box (provided)
with DRY ICE
Ship in cooler with DRY ICE
Ship in cooler with wet ice
(preferred but not required)
Ship in padded envelope
Ship in cooler with DRY ICE
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