United States    Office of Water    EPA- 820R15100
          Environmental   Mail Code 4304T   June 2015
          Protection Agency
Drinking Water Health Advisory
     for the Cyanobacterial
       Microcystin Toxins

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     Drinking Water Health Advisory
for the Cyanobacterial Microcystin Toxins
                  Prepared by:

        U.S. Environmental Protection Agency
              Office of Water (43 04T)
        Health and Ecological Criteria Division
              Washington, DC 20460
         EPA Document Number: 820R15100
               Date: June 15,2015

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                               ACKNOWLEDGMENTS
This document was prepared by U.S. EPA Scientists Lesley V.  D'Anglada, Dr.P.H. (lead) and
Jamie Strong, Ph.D. Health and Ecological Criteria Division, Office of Science and Technology,
Office of Water. EPA gratefully acknowledges the valuable contributions from Health Canada's
Water and Air Quality Bureau, in developing the Analytical Methods and Treatment Technologies
information included in this document.

This Health Advisory was provided for review and comments were received from staff in the
following U.S. EPA Program Offices:
      U.S. EPA Office of Ground Water and Drinking Water
      U.S. EPA Office of Science and Technology
      U.S. EPA Office of Research and Development
      U.S. EPA Office of Children's Health Protection
      U.S. EPA Office of General Counsel

This Health Advisory was provided for review and comments were received from the following
other federal and health agencies:
      Health Canada
      U.S. Department of Health and Human Services, Centers for Disease Control and
      Prevention
               Drinking Water Health Advisory for Microcystins-June 2015

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                               TABLE OF CONTENTS

ACKNOWLEDGMENTS	I
TABLE OF CONTENTS	II
LIST OF TABLES	IV
LIST OF FIGURES	IV
ABBREVIATIONS AND ACRONYMS	V
EXECUTIVE SUMMARY	1
1.0    INTRODUCTION AND BACKGROUND	3
   1.1    Current Criteria, Guidance and Standards	3
2.0    PROBLEM FORMULATION	6
  2.1    Cyanobacteria and Production of Microcystins	6
  2.2    Physical and Chemical Properties	6
  2.3    Sources and Occurrence	9
    2.3.1   Occurrence in Surface Water	10
    2.3.2   Occurrence in Drinking Water	13
  2.4    Environmental Fate	14
    2.4.1   Persistence	14
    2.4.2   Mobility	15
  2.5    Nature of the Stressor-Characteristics of the Microcystin Toxins	15
    2.5.1   Toxicokinetics	15
    2.5.2   Noncancer Health Effects Data	16
       2.5.2.1   Human Studies	16
       2.5.2.2   Animal Studies	17
    2.5.3   Mode of Action for Noncancer Health Effects	18
    2.5.4   Carcinogenicity Data	18
  2.6    Conceptual Model for Microcystins	19
    2.6.1   Conceptual Model Diagram	20
    2.6.2   Factors Considered in the Conceptual Model for Microcystins	22
  2.7    Analysis Plan	23
3.0    HEALTH EFFECTS ASSESSMENT	26
  3.1    Dose-Response	26
    3.1.1   Study Selection	26
    3.1.2   Endpoint Selection	28
  3.2    Ten-day Health Advisory	28
    3.2.1   Bottle-fed Infants and Young  Children of Pre-school Age	28
    3.2.2   School-age Children through Adults	29
    3.2.3   Uncertainty Factor Application	29
4.0    RISK CHARACTERIZATION	31
  4.1    Use of microcystin-LR as a surrogate for total microcystins	31
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  4.2    Consideration of Study Duration	31
  4.3    Consideration of Reproductive Effects asEndpoint	32
  4.4    Allometric Scaling Approach	33
  4.5    Benchmark Dose (BMD) Modeling Analysis	33
  4.6    Carcinogenicity Evaluation	33
  4.7    Uncertainty and Variability	34
  4.8    Susceptibility	35
  4.9    Distribution of Body Weight and Drinking Water Intake by Age	35
  4.10   Distribution of Potential  Health Advisory Values by Age	36
5.0    ANALYTICAL METHODS	38
6.0    TREATMENT  TECHNOLOGIES	41
  6.1    Management and Mitigation of Cyanobactedal Blooms in Source Water	41
  6.2    Drinking Water Treatment	42
     6.2.1  Conventional Treatment for Microcystins	43
     6.2.2  Adsorption	44
     6.2.3  Chemical Oxidation	45
     6.2.4  Other Filtration Technologies	46
     6.2.5  Combined Treatment Technologies	47
  6.3    Point-of-Use (POU) Drinking Water Treatment Units	48
7.0    REFERENCES	49
               Drinking Water Health Advisory for Microcystins-June 2015            iii

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                                   LIST OF TABLES

Table 1-1. International Guideline Values for Microcystins	4
Table 1-2. State Guideline Values for Microcystins	5
Table 2-1. Abbreviations for Microcystins (Yuan et al., 1999)	8
Table 2-2. Chemical and Physical Properties of Microcystin-LR	9
Table 2-3. States surveyed as part of the 2007 National Lakes Assessment with water body
    Microcystin concentrations above the WHO advisory guideline level for recreational water
    of 10|ig/L(U.S. EPA, 2009)	11
Table 3-1. Liver Weights and Serum Enzyme Levels in Rats Ingesting Microcystin-LR in
    Drinking Water (Heinze, 1999)	27
Table 3-2. Histological Evaluation of the Rat Livers after Ingesting Microcystin-LR in Drinking
    Water (Heinze, 1999)	27
                                  LIST OF FIGURES

Figure 2-1. Structure of Microcystin (Kondoetal., 1992)	7
Figure 2-2. Structure of the amino acids Adda and Mdha (Harada et al., 1991)	8
Figure 2-3. Conceptual Model of Exposure Pathways to Microcystins in Drinking Water	21
Figure 4-1. 90th Percentile Drinking Water Ingestion Rates by Age Group	35
Figure 4-2. Ten-day Health Advisories for Microcystins by Age Group	37
               Drinking Water Health Advisory for Microcystins-June 2015            iv

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                        ABBREVIATIONS AND ACRONYMS
rgt
A
Adda
ALT
ALP
AST
AWWARF
BMD
BMDL
BW
C102
CAS
CASA
CCL
CWA
DBF
DL
EBCT
ELISA
EPA
FSH
g
GC/MS
GAC
GLERL
H202
HA
HAB
HESD
HPLC
IARC
i.p.
Kg
L
LC/MS
LDH
LD50
LH
LOAEL
MC-LA
MC-LR
MC-RR
MC-YR
MC-YM
F-Glutamyltransferase
Alanine
3-Amino-9-Methoxy-2,-6,-8-,Trimethyl-10-Phenyldeca-4,-6-Dienoic Acid
Alanine Aminotransferase
Alkaline Phosphatase
Aspartate Aminotransferase
American Water Works Association Research Foundation
Benchmark Dose
Benchmark Dose Level
Body Weight
Chlorine Dioxide
Chemical Abstracts Service
Computer-Assisted Sperm Analysis
Contaminant Candidate List
Clean Water Act
Disinfection By-Products
Detection Limit
Empty Bed Contact Time
Enzyme-Linked Immunosorbent Assay
U.S. Environmental Protection Agency
Follicle Stimulating Hormone
Gram
Gas Chromatograph/Mass Spectrometry
Granular Activated Carbon
Great Lakes Environmental Research Laboratory
Hydrogen Peroxide
Health Advisory
Harmful Algal Bloom
Health Effects Support Document
High-Performance Liquid Chromatography
International Agency for Research on Cancer
Intraperitoneal
Kilogram
Leucine
Liquid Chromatography/Mass Spectrometry
Lactate Dehydrogenase
Lethal Dose to 50% of Organisms
Luteinizing Hormone
Lowest-Observed-Adverse-Effect Level
Microcystin-LA
Microcystin-LR
Microcystin-RR
Microcystin-YR
Microcystin-YM
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Mdha
MERHAB-LGL

US
LOQ
Mdls
mg
ml
MMPB
MOA
MF
MWCO
NDEA
NF
NLA
NOAA
NOAEL
NOD
NOM
OATp
PAC
PAS
PBS
PDA
P-GST
POD
POU
PP2
PP1
PPIA
RfD
RO
ROS
SDWA
SPE
TEF
TOC
TOXLINE
TUNEL

UF
UF
USGS
UV
WHO
Methyl dehy droal anine
Monitoring and Event Response to Harmful Algal Blooms in the Lower
Great Lakes
Microgram
Micromole
Level of Quantification
Method Detection Limit
Milligram
Milliliter
2-methyl-3-methoxy-4-phenylbutyric acid
Mode of Action
Microfiltration
Molecular Weight Cut-Off
N-Nitrosodiethylamine
Nanofiltration
National Lakes Assessment
National Oceanic and Atmospheric Administration
No-Observed-Adverse-Effect Level
Nodularin
Natural Organic Material
Organic Acid Transporter Polypeptides
Powdered Activated Carbon
Periodic Acid-Schiff
Phosphate-Buffered Saline
Photodiode Array Detector
glutathione S-transferase placental form-positive
Point of Departure
Point-of-Use
Protein Phosphatase 2A
Protein Phosphatase 1
Protein Phosphatase Inhibition Assays
Reference Dose
Reverse Osmosis
Reactive Oxygen Species
Safe Drinking Water Act
Solid-Phase Extraction
Toxicity Equivalency Factors
Total Organic Carbon
Toxicology Literature Online
Terminal Deoxynucleotidyl Transferase-Mediated dUTP-Biotin Nick End-
Labeling Assay
Uncertainty Factor
Ultrafiltration
United States Geological Survey
Ultraviolet
World Health Organization
               Drinking Water Health Advisory for Microcystins-June 2015
                                                             VI

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                                EXECUTIVE SUMMARY

       Microcystins are toxins produced by a number of cyanobacteria species, including
members ofMicrocystis, Anabaena, Nodularia, Nostoc,  Oscillatoria, Fischerella, Planktothrix,
and Gloeotrichia. Approximately 100 microcystin congeners exist, which vary based on amino
acid composition. Microcystin-LR is one of the most potent congeners and the majority of
toxicological data on the effects of microcystins are available for this congener.

       Many environmental factors such as the ratio of nitrogen to phosphorus, temperature,
organic matter availability, light attenuation and pH play an important role in the development of
microcystin blooms, both in fresh and marine water systems and could encourage toxin
production. Microcystins are water soluble and tend to remain contained within the cyanobacterial
cell (intracellular), until the cell breaks and they are released into the water (extracellular).

       This Health Advisory (HA) for microcystins is focused on drinking water as the primary
source of exposure.  Exposure to cyanobacteria and their toxins may  also occur by ingestion of
toxin-contaminated  food, including consumption offish, and by inhalation and dermal contact
during bathing or showering and during recreational activities in waterbodies with the toxins.
While these types of exposures cannot be quantified at this time, they are assumed to contribute
less to the total cyanotoxin exposures than ingestion of drinking water. Due to the seasonality of
cyanobacterial blooms, exposures are not expected to be chronic.

       Limited data in humans and animals demonstrate the absorption of microcystins from the
intestinal tract and distribution to the liver, brain, and other tissues. Elimination from the body
requires facilitated transport using receptors belonging to the Organic Acid Transporter
polypeptide (OATp) family. Data for humans and other mammals suggest that the liver is a
primary site for binding these proteins (i.e., increased liver weight in laboratory animals and
increased serum enzymes in laboratory animals and humans). Once inside the cell, these toxins
covalently bind to cytosolic proteins (PP1 and PP2) resulting in their retention in the liver.
Limited data are available on the metabolism of microcystins, but most of the studies indicate that
microcystins can be conjugated with glutathione and cysteine to increase their solubility and
facilitate excretion.

       The main source of human health effects data for microcystins is from acute recreational
exposure to cyanobacterial blooms. Symptoms include headache, sore throat, vomiting and
nausea, stomach pain,  dry cough, diarrhea, blistering around the mouth, and pneumonia.
However, human  data on the oral toxicity of microcystins are limited and confounded by:
potential co-exposure to other contaminants; a lack of quantitative information; and other
confounding factors. Reports of human intravenous exposure to dialysate prepared with
microcystin-contaminated water indicated acute liver failure and death in a large number of the
exposed patients.

       Studies in laboratory animals demonstrate liver, kidney, and  reproductive effects
following short-term and subchronic oral exposures to microcystin-LR. Studies evaluating the
chronic toxicity of microcystins have not shown clinical signs of toxicity and are limited by study
design and by the lack of quantitative data.
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       The U.S. Environmental Protection Agency (EPA) identified a study by Heinze (1999)
conducted on rats as the critical study used in the derivation of the reference dose (RfD) for
microcystins. The critical effects identified in the study are increased liver weight, slight to
moderate liver lesions with hemorrhages, and increased enzyme levels as a result of exposure to
microcystin-LR. The lowest-observed-adverse-effect level (LOAEL) was determined to be 50
ug/kg/day, based on these effects. The drinking water route of exposure matches  potential
drinking water exposure scenarios in humans. The total uncertainty factor (UF) applied to the
LOAEL was 1000. This was based on a UF of 10 for intraspecies variability, a UF of 10  for
interspecies variability, a UF of 3 (101/2) for extrapolation from a LOAEL to no-observed-adverse-
effect level (NOAEL), and a UF of 3 (101/2) to account for deficiencies in the database. EPA is
using microcystin-LR as a surrogate for other microcystin congeners. Therefore,  the HA based on
this critical study applies to total microcystins.

       EPA is issuing a Ten-day HA  for microcystins based on the Heinze (1999) short-term, 28-
day study. Studies of a duration of 7 to 30 days are typically used to derive Ten-day HAs. The HA
is consistent with this duration and appropriately matches human  exposure scenarios for
microcystins in drinking water. Cyanobacterial blooms are usually seasonal, typically occurring
from May through October. Microcystins typically have a half-life of 4 days to 14 days in surface
waters, (depending on the degree of sunlight, natural organic matter, and the presence of bacteria)
and can be diluted via transport. In addition, concentrations in finished drinking water can be
reduced by drinking water treatment and management measures.

       The Ten-day HA value for bottle-fed infants and young children of pre-school age is 0.3
|ig/L and for school-age children through adults is 1.6 |ig/L for microcystins. The two advisory
values use the same toxicity data (RfD) and represent differences in drinking water intake and
body weight for different life stages. The first advisory value is based on the summation  of the
time-weighted drinking water intake/body weight ratios for birth to <12  months of age. The
second advisory value is based on  the mean body weight and 90th percentile  drinking water
consumption rates for adults age 21 and over (U.S. EPA's Exposure Factors  Handbook (201 la)),
which is similar to that of school-aged children. Populations such as pregnant women and nursing
mothers, the elderly, and immune-compromised individuals or those receiving  dialysis treatment
may be more  susceptible than the general population to the health effects of microcystins. As a
precautionary measure, individuals that fall into these susceptible groups may want to consider
following the recommendations for children pre-school age and younger. This  HA is not a
regulation, it is not legally enforceable, and it does not confer legal rights or impose legal
obligations on any party.

       Applying the U.S. EPA (2005) Guidelines for Carcinogen Risk Assessment, there is
inadequate information to assess carcinogenic potential of microcystins. The few available
epidemiological studies are limited by their study design,  poor measures of exposure, potential
co-exposure to other contaminants, and the lack of control for confounding factors. No long term
animal studies were available to evaluate dose-response for the tumorigenicity  of microcystins
following lifetime exposures.  Other studies evaluating the tumor promotion potential of
microcystin found an increase in the number and/or  size of GST-P positive foci observed. In two
promotion studies, microcystin-LR alone showed no initiating activity.
                Drinking Water Health Advisory for Microcystins-June 2015

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1.0 INTRODUCTION AND BACKGROUND

       EPA developed the non-regulatory Health Advisory (HA) Program in 1978 to provide
information for public health officials or other interested groups on pollutants associated with
short-term contamination incidents or spills for contaminants that can affect drinking water
quality, but are not regulated under the Safe Drinking Water Act (SDWA). At present, EPA lists
HAs for 213 contaminants (http://water.epa.gov/drink/standards/hascience.cfm).

       HAs identify the  concentration of a contaminant in drinking water at which adverse health
effects are not anticipated to occur over specific exposure durations (e.g., one-day, ten-days, and a
lifetime). HAs serve as informal technical guidance to assist Federal, State and local officials, and
managers of public or community water systems in protecting public health when emergency
spills or contamination situations occur. An HA provides information on the environmental
properties, health effects, analytical methodology,  and treatment technologies for removal of
drinking water contaminants.

     The Health Effects  Support Document for Microcystim (U.S.EPA, 2015 a) is the peer-
reviewed, effects assessment that supports this HA. This document  is available at
http://www2.epa.gov/nutrient-policy-data/health-and-ecological-effects. The HAs are not legally
enforceable Federal standards and are subject to change as new information becomes available.
The structure of this Health Advisory is consistent with EP A's Framework for Human Health
Risk Assessment to Inform Decision Making (U.S.EPA, 2014).

       EPA is releasing  the Recommendations for Public Water Systems to Manage Cyanotoxins
in Drinking Water (U.S.  EPA, 2015b) as a companion to the HAs for microcystins and
cylindrospermopsin. The document is intended to assist public drinking water systems (PWSs)
that choose to develop system-specific plans for evaluating their source waters for vulnerability to
contamination by microcystins and cylindrospermopsin. It is designed to provide information and
a framework that PWSs and others as appropriate may consider to inform their decisions on
managing the risks from  cyanotoxins in drinking water.
1.1     Current Criteria, Guidance and Standards

       Currently there are no U.S. federal water quality criteria, or regulations for cyanobacteria
or cyanotoxins in drinking water under the SDWA or in ambient waters under the Clean Water
Act (CWA). The Safe Drinking Water Act (SDWA), as amended in 1996, requires the EPA to
publish a list of unregulated contaminants every five years that are not subject to any proposed or
promulgated national primary drinking water regulations, which are known or anticipated to occur
in public water systems, and which may require regulation. This list is known as the Contaminant
Candidate List (CCL). The EPA's Office of Water included cyanobacteria and cyanotoxins on the
first and second CCL (CCL 1, 1998; CCL 2, 2005). EPA included cyanotoxins, including
anatoxin-a, cylindrospermopsin, and microcystin-LR, on CCL 3 (2009) and the draft CCL 4
(April 2015 for consideration).
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        SDWA requires the Agency to make regulatory determinations on at least five CCL
 contaminants every five years. When making a positive regulatory determination, EPA
 determines whether a contaminant meets three criteria:

        •  The contaminant may have an adverse effect on the health of persons,
        •  The contaminant is known to occur or there is substantial likelihood the contaminant
           will occur in public water systems with a frequency and at levels of concern, and
        •  In the sole judgment of the Administrator, regulating the contaminant presents a
           meaningful opportunity for health risk reductions.

        To make these determinations, the Agency uses data to analyze occurrence (prevalence
 and magnitude) and health effects. EPA continues gathering this information to inform future
 regulatory determinations for cyanotoxins under the SDWA. The SDWA also provides the
 authority for EPA to publish non-regulatory HAs or take other appropriate actions for
 contaminants not subject to any national primary drinking water regulation. EPA is providing this
 HA and the HA for cylindrospermopsin to assist State and local officials in evaluating risks from
 these contaminants in drinking water.

        Internationally, eighteen countries and three U.S. states have developed drinking water
 guidelines for microcystins, as shown in Table 1.1 and Table 1.2, respectively, based on lifetime
 exposures.
 Table 1-1. International Guideline Values for Microcystins
             Country
  Guideline Value
            Source
    Brazil,  China, Czech Republic,
 Denmark, Finland, France, Germany,
   Italy, Japan, Korea, Netherlands,
   Norway, New Zealand, Poland,
	South Africa, and Spain	
       1.0 ug/L
     microcystin-LR
Based on the World Health
Organization (WHO) Provisional
Guideline Value of lug/L for
drinking water
(WHO,  1999; 2003)	
             Australia
1.3 ug/L microcystin-
    LR (toxicity
    equivalents)
   Australian Drinking Water
         Guidelines 6
   (NHMRC, NRMMC, 2011)
              Canada
      1.5 ug/L
   microcystin-LR
    Guidelines for Canadian
    Drinking Water Quality:
   Supporting Documentation
    Cyanobacterial Toxins-
        Microcystin-LR
     (Health Canada, 2002)
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Table 1-2. State Guideline Values for Microcystins
State
Minnesota
Ohio
Oregon
Guideline Value
0.04 |ig/L Microcystin-LR
1 ng/L Microcystin
1 |ig/L Microcystin-LR
Source
Minnesota Department of Health (MDH, 2012)
Public Water System Harmful Algal Bloom
Response Strategy (Ohio EPA, 2014)
Public Health Advisory Guidelines, Harmful Algae
Blooms in Freshwater Bodies. (OHA, 2015)
       For drinking water, the provisional WHO Guideline value for microcystin-LR of 1 ug/L
(or the underlying Tolerable Daily Intake (TDI) of 0.04 ug/kg) has been widely used as the basis
for national standards or guideline values (WHO,  1999, 2003). Following the release of the WHO
provisional guideline, drinking-water standards or national guideline values were adopted in 16
countries. Australia and Canada have used the TDI, but have adapted other factors in the
calculation to reflect their national circumstances  (e.g. body weight or amounts of water
consumed), thus reaching somewhat higher guidance values or standards (Chorus, 2012). A few
countries have issued guideline values specifically for microcystin-LR while others use
microcystin-LR as a surrogate for all microcystin  congeners (i.e. toxicity equivalents). Values are
similar across all countries, ranging between 1.0 and  1.5 ug/L based on lifetime exposures.
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2.0 PROBLEM FORMULATION

     The development of the HA begins with problem formulation, which provides a strategic
framework by focusing on the most relevant cyanotoxin properties and endpoints identified in the
Health Effects Support Document for Microcystim (U.S. EPA, 2015 a).

2.1     Cyanobacteria and Production of Microcystins

       Cyanobacteria, formerly known as blue-green algae (Cyanophyceae), are a group of
bacteria with chlorophyll-a capable of photosynthesis (light and dark phases) (Castenholz and
Waterbury, 1989). Most Cyanobacteria are aerobic photoautotrophs, requiring only water, carbon
dioxide, inorganic nutrients and light for survival, while others have heterotrophic properties and
can survive long periods in complete darkness (Fay, 1965). Some species are capable of nitrogen
fixation (diazotrophs) (Duy et al., 2000), producing inorganic nitrogen compounds for the
synthesis of nucleic acids and proteins. Cyanobacteria can form symbiotic associations with
animals and plants, such as fungi, bryophytes, pteriodophytes, gymnosperms and angiosperms
(Rai, 1990), supporting their growth and reproduction (Sarma, 2013; Hudnell, 2008; Hudnell,
2010).

       Under the right conditions of pH, nutrient availability, light, and temperature,
Cyanobacteria can reproduce quickly forming a bloom. Although studies of the impact of
environmental factors on cyanotoxin production are ongoing, nutrient (N, P and trace metals)
supply rates, light, temperature, oxidative stressors, interactions with other biota (viruses, bacteria
and animal grazers), and most likely, the combined effects of these factors are all involved (Paerl
and Otten 2013a; 2013b). Fulvic and humic acids reportedly encourage Cyanobacteria growth
(Kosakowska et al., 2007).

       Microcystins are produced by several cyanob acted al species, including Anabaena,
Fischerella, Gloeotrichia, Nodularia, Nostoc, Oscillatoria., members ofMicrocystis, and
Planktothrix (Duy et al., 2000;  Codd et al., 2005; Stewart et al., 2006a; Carey et al., 2012).
2.2     Physical and Chemical Properties

       The cyclic peptides include around 100 congeners of microcystins. Table 2-1 lists only the
most common microcystins congeners. Figure 2-1 provides the structure of microcystin where X
and Y represent variable amino acids. Although substitutions mostly occur in positions X and Y,
other modifications have been reported for all of the amino acids (Puddick et al., 2015). The
amino acids are joined end-to-end and then head to tail to form cyclic compounds that are
comparatively large (molecular weights ranging from -800 to 1,100 g/mole).
                Drinking Water Health Advisory for Microcystins-June 2015

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                 Figure 2-1. Structure of Microcystin (Kondo et al., 1992)
                                                            C02H
       Microcystin congeners vary based on their amino acid composition and through
methylation or demethylation at selected sites within the cyclic peptide (Duy et al., 2000). The
variations in composition and methylation account for the large number of toxin congeners. The
microcystins are named based on their variable amino acids, although they have had many other
names (Carmichael et al., 1988). For example, microcystin-LR, the most common congener,
contains leucine (L) and arginine (R) (Carmichael, 1992). The letters used to identify the variable
amino acids are the standard single letter abbreviations for the amino acids found in proteins. The
variable amino acids are usually the L-amino acids as found in  proteins. In this HA, the term
microcystin may be followed by the abbreviations for the variable amino acids. For example,
microcystin-LR is for the microcystin with leucine in the X position of Figure 2-1 and arginine in
the Y position. Most research has concentrated on microcystin-LR, with lesser amounts of data
available for the other amino acid combinations. For the purpose of this HA, microcystin-LR is
used as the surrogate for total microcystins.

       Structurally, the microcystins are monocyclic heptapeptides that contain seven amino
acids: two variable L-amino acids, three common D-amino acids or their derivatives, and two
novel D-amino acids. These two D-amino acids are:  3S-amino-9S-methoxy-2,6,8S,-trimethyl-10-
phenyldeca-4,6-dienoic acid (Adda) and methyldehydroalanine (Mdha). Adda is characteristic of
all toxic microcystin structural congeners and is essential for their biological activity (Rao et  al.,
2002; Funari and Testai, 2008). Mdha plays  an important role in the ability of the microcystins to
inhibit protein phosphatases. Figure 2-2 illustrates the  structures of these two unique amino acid
microcystin components.

       Microcystins are water soluble. In aquatic environments, the cyclic peptides tend to
remain contained within the cyanobacterial cell and  are released in substantial amounts only upon
cell lysis. The microcystins are most frequently found in cyanobacterial blooms in fresh and
brackish waters (WHO, 1999). Table 2-2 provides chemical and physical properties of
microcystin-LR.
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Table 2-1. Abbreviations for Microcystins (Yuan et al., 1999)
Microcystin Congeners
Microcystin-LR
Microcystin-RR
Microcystin-YR
Microcystin-LA
Microcystin-LY
Microcystin-LF
Microcystin-LW
Amino Acid in X
Leucine
Arginine
Tyrosine
Leucine
Leucine
Leucine
Leucine
Amino Acid in Y
Arginine
Arginine
Arginine
Alanine
Tyrosine
Phenylalanine
Tryptophan
      Figure 2-2. Structure of the amino acids Adda and Mdha (Harada et al., 1991).
                20
                                                         CH    0
                                                          H2C
                                                            3
                                Adda
Mdha
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Table 2-2. Chemical and Physical Properties of Microcystin-LR
Property
Chemical Abstracts Registry (CAS) #
Chemical Formula
Molecular Weight
Color/Physical State
Boiling Point
Melting Point
Density
Vapor Pressure at 25°C
Henry's Law Constant
J^-OW
Koc
Solubility in Water
Other Solvents
Microcystin-LR
101043-37-2
C49H?4NloOl2
995.17g/mole
Solid
N/A
N/A
1.29g/cm3
N/A
N/A
N/A
N/A
Highly
Ethanol and methanol
          Sources: Chemical Book, 2012; TOXLINE, 2012
2.3
Sources and Occurrence
       Cyanotoxin production is strongly influenced by the environmental conditions that
promote growth of particular cyanobactedal species and strain. Nutrient concentrations, light
intensity, water turbidity, temperature, competing bacteria and phytoplankton, pH, turbulence,
and salinity are all factors that affect cyanobacterial growth and change in cyanobacteria
population dynamics. Although environmental conditions affect the formation of blooms, the
numbers of cyanobacteria and toxin concentrations produced are not always closely related.
Cyanotoxin concentrations depend on the dominance and diversity of strains within the bloom
along with environmental and ecosystem influences on bloom dynamics (Hitzfeld et al., 2000;
Chorus et al., 2000; WHO, 1999). Extracellular microcystins (either dissolved in water or bound
to other materials) typically make up less than 30% of the total microcystin concentration in
source water (Graham et al., 2010). Most of the toxin is intracellular, and released into the water
when the cells rupture or die. Both intracellular and extracellular microcystins may also be
present in treated water, depending on the type of treatment processes in place.
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2.3.1       Occurrence in Surface Water

       Microcystins are the most common cyanotoxin found worldwide and have been reported
in surface waters in most of the U.S. and Europe (Funari and Testai, 2008). Dry-weight
concentrations of microcystins in surface freshwater cyanobactedal blooms or surface freshwater
samples reported worldwide between 1985 and 1996 ranged from 1 to 7,300 |ig/g. Water
concentrations of extracellular plus intracellular microcystins ranged from 0.04 to 25,000  |ig/L.
The concentration of extracellular microcystins ranged from 0.02 to a high of 1,800 |ig/L reported
following treatment of a large cyanobacteria bloom with algaecide (WHO, 1999) and the U.S.
Geological Survey (USGS) reported a concentration of 150,000 |ig/L total microcystins, in a lake
in Kansas (Graham et al., 2012).

       According to a survey conducted in Florida in 1999 between the months of June and
November, the most frequently observed cyanobacteria wereMicrocystis (43.1%),
Cylindrospermopsis (39.5%), andAnabaena spp (28.7%)  (Burns, 2008). Of 167 surface water
samples taken from 75 waterbodies, 88 samples were positive for cyanotoxins. Microcystin was
the most commonly found cyanotoxin in water samples collected, occurring in 87 water samples.

       In 2002, the Monitoring and Event Response to Harmful Algal Blooms in the Lower Great
Lakes (MERHAB-LGL) project evaluated the occurrence  and distribution of cyanobacterial
toxins in the lower Great Lakes region (Boyer, 2007). Analysis for total microcystins was
performed using Protein Phosphatase Inhibition Assay (PPIA). Microcystins were detected in at
least 65% of the samples, mostly in Lake Erie, Lake Ontario, and Lake Champlain. The National
Oceanic and Atmospheric Administration (NOAA) Center of Excellence for Great Lakes and
Human Health (CEGLHH) continues to monitor the Great Lakes and regularly samples algal
blooms for microcystin in response to bloom events.

       A 2004 study of the Great Lakes found high levels of cyanobacteria during the month of
August (Makarewicz et al., 2006). Microcystin-LR was analyzed by PPIA (limit of detection of
0.003 |ig/L) and was detected at levels of 0.084 ug/L in the nearshore and 0.076 ug/L in the bays
and rivers. This study reported higher levels of microcystin-LR (1.6 to 10.7ug/L) in smaller lakes
in the Lake Ontario watershed.

       In 2006, the USGS conducted a study of 23 lakes in the Midwestern U.S. in which
cyanobacterial blooms were sampled to determine the co-occurrence of toxins in cyanobacterial
blooms (Graham et al., 2010). This study reported that microcystins were detected in 91% of the
lakes sampled. Mixtures of all the microcystin congeners measured (LA, LF, LR, LW, LY, RR,
and YR) were common and all the congeners were present in association with the blooms.
Microcystin—LR and -RR were the dominant congeners detected with mean concentrations of
104 and 910 ug/L, respectively.

       EPA's National Aquatic Resource Surveys (NARS) generate national estimates of
pollutant occurrence every 5 years.  In 2007, the National Lakes Assessment (NLA) conducted the
first-ever national probability-based survey of the nation's lakes, ponds and reservoirs (U.S.EPA,
2009). This baseline study of the condition of the nation's lakes provided estimates of the
condition of natural and man-made freshwater lakes, ponds, and reservoirs greater than 10 acres
and at least one meter deep. A total of 1,028 lakes were sampled  in the NLA during the summer


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of 2007. The NLA measured microcystins using Enzyme Linked Immunosorbent Assays (ELISA)
with a detection limit of 0.1 jig/L as well as cyanob acted al cell counts and chlorophyll-a
concentrations, which were indicators of the presence of cyanob acted al toxins. Samples were
collected in open water at mid-lake. Due to the design of the survey, no samples were taken
nearshore or in other areas where scums were present.

       A total of 48 states were sampled in the NLA, and states with lakes reporting microcystins
levels above the WHO's moderate risk1 threshold in recreational water (>10 |ig/L) are shown in
Table 2-3. Microcystins were present in 30% of the lakes sampled nationally, with sample
concentrations that ranged from the limit of detection (0. 1 |ig/L) to 225 |ig/L. Two states (North
Dakota and Nebraska),  had 9% of samples above 10 |ig/L. Other states including Iowa, Texas,
South Dakota, and Utah also had samples that exceeded 10 |ig/L. Several samples in North
Dakota, Nebraska, and  Ohio  exceeded the WHO high risk threshold value for recreational waters
of 20 |ig/L (192 and 225 |ig/L, respectively). EPA completed a second survey of lakes in 2012,
but data have not yet been published.

       Microcystins have been detected in most of the states of the  U.S., and over the years many
studies have been done to determine their occurrence in surface water. USGS, for example, did a
study in the Upper Klamath Lake in Oregon in 2007 and detected total microcystin concentrations
between 1 |ig/L and 17 |ig/L (VanderKooi et al., 2010). USGS also  monitored Lake Houston in
Texas from 2006 to 2008, and found microcystins in 16% of samples with concentrations less
than or equal to 0.2 |ig/L (Beussink and Graham, 201 1). In 201 1, USGS conducted a study on the
upstream reservoirs of the Kansas River, a primary source of drinking water for residents in
northeastern Kansas, to characterize the transport of cyanobacteria and associated compounds
(Graham et al., 2012). Concentrations of total microcystin were low in the majority of the
tributaries with the exception of Milford Lake, which had higher total microcystin concentrations,
some exceeding the Kansas recreational guidance level of 20 |ig/L.  Upstream from Milford Lake,
a cyanob acted al bloom was observed with a total microcystin  concentration of 150,000 |ig/L.
When sampled a week later, total microcystin concentrations were less than 1 |ig/L. The study
authors indicated that this may be due to dispersion of microcystins  through the water column or
to other areas, or by degradation of microcystins via abiotic and biological processes. Samples
taken during the same time from outflow waters contained total microcystin concentrations of 6.2
       In 2005, Washington State Department of Ecology developed the Ecology Freshwater
Algae Program to focus on the monitoring and management of cyanobacteria in Washington
lakes, ponds, and streams (WSDE, 2012). The data collected have been summarized in a series of
reports for the  Washington State Legislature (Hamel, 2009, 2012). Microcystin levels ranged
from the detection limit (0.05  |ig/L) to 4,620 |ig/L in 2008, 18,700 |ig/L in 2009, 853 |ig/L in
20 1 0, and 26,400  |ig/L in 20 1  1 .
1 The WHO established guideline values for recreational exposure to cyanobacteria using a three-tier approach: low
risk (<20,000 cyanobacterial cells/ml corresponding to <10 ug/L of MC-LR); moderate risk (20,000-100,000
cyanobacterial cells/ml corresponding to 10-20 ug/L of MC-LR); and high risk (>100,000 cyanobacterial cells/ml
corresponding to >20 ug/L for MC-LR).


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Table 2-3. States Surveyed as Part of the 2007 National Lakes Assessment with Water Body
Microcystins Concentrations above the WHO Advisory Guideline Level for Recreational
Water of 10 ug/L (U.S. EPA, 2009)
State
North Dakota
Nebraska
South Dakota
Ohio
Iowa
Utah
Texas
Number
of Sites
Sampled
38
42
40
21
20
26
51
Percentage of Samples
with Detection of
Microcystins >10 ug/L
9.1%
9.1%
4.9%
4.5%
4.5%
3.6%
1.8%
Maximum Detection
of
Microcystins
192 |ig/L
225 |ig/L
33,ig/L
78 |ig/L*
38 |ig/L*
15 |ig/L*
28 |ig/L *
      Single Sample
       Other surveys and studies have been conducted to determine the occurrence of
microcystin in lakes in the United States. A survey conducted during the spring and summer of
1999 and 2000 in more than 50 lakes in New Hampshire found measureable microcystin
concentrations in all samples (Haney and Ikawa, 2000). Microcystins were analyzed by ELISA
and were found in all  of the lakes sampled with a mean concentration of 0.1  |ig/L. In 2005 and
2006, a study conducted in New York, including Lake Ontario, found variability in microcystin-
LR concentrations within the Lake Ontario ecosystem (Makarewicz et  al., 2009). Of the samples
taken in Lake Ontario coastal waters, only 0.3% of the samples exceeded the WHO provisional
guideline value for drinking water of 1 |ig/L. However, 20.4% of the samples taken at upland
lakes and ponds within the Lake Ontario watershed, some of them sources of drinking water,
exceeded 1 |ig/L. During 2008 and 2009, a study was conducted  in Kabetogama Lake, Minnesota
which detected microcystin concentrations in association with algal blooms (Christensen et al.,
2011). Microcystin concentrations were detected in 78% of bloom samples. Of these, 50% were
above 1 ug/L, and two samples were above the high risk WHO recreational level of 20 ug/L.

       A study from 2002 evaluated water quality including chlorophyll-a concentration,
cyanobacterial assemblages, and microcystin concentrations in 11 potable water supply reservoirs
within the North Carolina Piedmont during dry summer growing seasons (Touchette et al., 2007).
Microcystins concentrations were assessed using ELISA. The study found that cyanobacteria
were the dominant phytoplankton community, averaging 65-95% of the total phytoplankton cells.
Although microcystin concentrations were detected in nearly all  source water samples,
concentrations were <0.8 ug/L.

       Since 2007, Ohio EPA (OHEPA, 2012) has been monitoring inland lakes for cyanotoxins.
Of the 19 lakes in Ohio sampled during the NLA,  36% had detectable levels of microcystins. In
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2010, OHEPA sampled Grand Lake St. Marys for anatoxin-a, cylindrospermopsin, microcystins,
and saxitoxin. Toxin levels ranged from below the detection limit (<0.15 ug/L) to more than
2,000 ug/L for microcystins. Follow-up samples taken in 2011 for microcystins indicated
concentrations exceeding 50 ug/L in August. During the same month, sampling in Lake Erie
found microcystins levels exceeding 100 ug/L.

       In 2008, NOAA began monitoring for cyanobactedal blooms in Lake Erie using high
temporal resolution satellite imagery. Between 2008 and 2010, Microcystis cyanobacterial blooms
were detected associated with water temperatures above 18°C (Wynne et al., 2013). Using the
Great Lakes Coastal Forecast System (GLCFS), forecasts of bloom transport are created to
estimate the trajectory of the bloom, and these are distributed  as bulletins to local managers,
health departments, researchers and other stakeholders. To evaluate bloom toxicity, the Great
Lakes Environmental Research Laboratory (GLERL) collected samples at six stations each week
for 24 weeks, measuring toxin concentrations as well as chlorophyll biomass and an additional 18
parameters (e.g., nutrients) to improve future forecasts of these blooms. In 2014, particulate toxin
concentrations, collected from 1 meter depth, ranged from below detection to 36.7
ug/L. Particulate toxin concentrations peaked in August, 2014 at all sites, with the Maumee Bay
site yielding the highest toxin concentration of the entire sampling period. Dissolved toxin
concentrations were collected at each site from September until November when the field season
ended. During the final months of sampling (October-November), dissolved toxin concentrations
were detected with peak concentrations of 0.8 ug/L (mean: 0.28 +/- 0.2 ug/L) whereas particulate
toxin concentrations were below detection limits on many dates, indicating that a majority of the
toxins (mean: 72% +/- 37%) were in the dissolved pool as the bloom declined in intensity.

       Concentrations of microcystins were detected during sampling in 2005 and 2006 in lakes
and ponds used as a source of drinking water within the Lake  Ontario watershed (Makarewicz et
al., 2009). A microcystin-LR concentration  of 5.07 ug/L was found in Conesus Lake, a source of
public water supply that provides drinking water to approximately 15,000 people. Microcystin-LR
was also detected at 10.716 ug/L in Silver Lake, a public drinking water supply for four
municipalities.
2.3.2       Occurrence in Drinking Water

       The occurrence of cyanotoxins in drinking water depends on their levels in the raw source
water and the effectiveness of treatment methods for removing cyanobacteria and cyanotoxins
during the production of drinking water. Currently, there is no program in place to monitor for the
occurrence of cyanotoxins at surface-water treatment plants for drinking water in the U.S.
Therefore, data on the presence or absence of cyanotoxins in finished drinking water are limited.

       The American Water Works Association Research Foundation (AWWARF) conducted a
study on the occurrence of cyanobacterial toxins in source and treated drinking waters from 24
public water systems in the United States and Canada in 1996-1998 (AWWARF, 2001). Of 677
samples tested, microcystin was found in 80% (539) of the waters sampled, including source and
treated waters. Only two samples of finished drinking water were above 1 ug/L. A survey
conducted in 2000 in Florida (Burns, 2008) reported that microcystins were the most commonly
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found toxin in pre- and post-treated drinking water. Finished water concentrations ranged from
below detection levels to 12.5 |ig/L.

       During the summer of 2003, a survey was conducted to test for microcystins in 33 U.S.
drinking water treatment plants in the northeastern and Midwestern U.S. (Haddix et al., 2007).
Microcystins were detected at low levels ranging from undetectable (<0.15 |ig/L) to 0.36 jig/L in
all 77 finished water samples.

       In August 2014, the city of Toledo, Ohio issued a "do not drink or boil advisory" to nearly
500,000 customers in response to the presence of total microcystins in the city's finished drinking
water at levels up to 2.50 |ig/L. The presence of the toxins was due to a cyanob acted al bloom
near Toledo's drinking water intake located on Lake Erie. The advisory was lifted two days later,
after treatment adjustments led to the reduction of the cyanotoxin concentrations to concentrations
below the WHO guideline value of 1 |ig/L in all samples from the treatment plant and distribution
system.
2.4     Environmental Fate

       Different physical and chemical processes are involved in the persistence, breakdown, and
movement of microcystins in aquatic systems as described below.
2.4.1       Persistence

       Microcystins are relatively stable and resistant to chemical hydrolysis or oxidation at or
near neutral pH. Elevated or low pH or temperatures above 30°C may cause slow
hydrolysis. Microcystin is not destroyed by boiling (Rao et al., 2002). In natural waters kept in the
dark, microcystins have been observed to persist for 21 days to 2-3 months in solution and up to 6
months in dry scum (Rapala et al., 2006;  Funari and Testai, 2008).

       In the presence of full sunlight, microcystins undergo photochemical breakdown, but this
varies by microcystin congener (WHO, 1999; Chorus et al., 2000). The presence of water-soluble
cell pigments, in particular phycobiliproteins, enhances this breakdown. Breakdown can occur in
as few as two weeks to longer than six weeks, depending on the  concentration of pigment and the
intensity of the light (Tsuji et al., 1993; 1995). According to Tsuji et al, microcystin-LR was
photodegraded with a half-life (time it takes half of the toxin to degrade) of about 5 days in the
presence of 5 mg/L  of extractable cyanobacterial pigment. Humic substances can also act as
photosensitizers and can increase the rate of microcystin breakdown in sunlight. In deeper or
turbid water, the breakdown rate is slower.

       Microcystins are susceptible to degradation by aquatic bacteria found naturally in rivers
and reservoirs (Jones et al.,  1994). Bacteria isolates ofArthrobacter, Brevibacterium,
Rhodococcus, Paucibacter,  and  various strains of the genus Sphingomonas (Pseudomonas) have
been reported to be capable of degrading microcystin-LR (de la Cruz et al., 2011; Han et al.,
2012). These degradative bacteria have also been found in sewage effluent (Lam et al., 1995),
lake water (Jones et al., 1994; Cousins et al., 1996; Lahti et al., 1997a), and lake  sediment (Rapala
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et al., 1994; Lahti et al., 1997b). Lam et al., in 1995 reported that the biotransformation of
microcystin-LR followed a first-order decay with a half-life of 0.2 to 3.6 days (Lam et al., 1995).
In a study done by Jones et al. (1994) with microcystin-LR in different natural surface waters,
microcystin-LR persisted for 3 days to 3 weeks; however, more than 95% loss occurred within 3
to 4 days. A study by Christoffersen et al., 2002, measured half-lives in the laboratory and in the
field of approximately 1 day, driven largely by bacterial aerobic metabolism. These researchers
found that approximately 90% of the initial amount of microcystin disappeared from the water
phase within 5 days, irrespective of the starting concentration. Other researchers (Edwards et al.,
2008) have reported half-lives of 4 to 14 days, with longer half-lives associated with a flowing
stream and shorter half-lives associated with lakes.
2.4.2       Mobility

       Microcystins may adsorb onto naturally suspended solids and dried crusts of
cyanobacteria. They can precipitate out of the water column and reside in sediments for months
(Han et al., 2012: Falconer, 1998). Ground water is generally not expected to be at risk of
cyanotoxin contamination, however, ground water under the direct influence of surface water can
be vulnerable. A study conducted by the USGS and the University of Central Florida determined
that microcystin and cylindrospermopsin did not sorb in sandy aquifers and were transported
along with ground water (O'Reilly et al., 2011). The  authors suggested that the removal of
microcystin was due to biodegradation.
2.5     Nature of the Stressor-Characteristics of the Microcystin Toxins
2.5.1       Toxicokinetics

       No data were available that quantified the intestinal, respiratory or dermal absorption of
microcystins. Available data indicate that the Organic Acid Transporter polypeptide (OATp)
receptors facilitate the absorption of toxins from the intestinal tract into liver, brain, and other
tissues. The OATp family transporters facilitate the cellular, sodium-independent uptake and
export of amphipathic compounds such as bile salts, steroids, drugs, peptides and toxins (Cheng et
al., 2005; Fischer et al., 2005; Svoboda et al., 2011). This facilitated transport is necessary for
both uptake of microcystins into organs and tissues as well as for their export. Microcystins
compete with bile acids for uptake by the liver and is limited in the presence of bile acids and
other physiologically-relevant substrates for the transporter (Thompson and Pace, 1992). Other
studies following in vitro or in vivo exposures have shown that inhibition of microcystin uptake
by its OATp transporter reduces or eliminates the liver toxicity observed (Runnegar et al., 1981,
1995; Runnegar and Falconer, 1982; Hermansky et al., 1990a, b).

       Limited information is available on the metabolism of microcystins. Some studies have
found that metabolism of microcystin-LR in mice occurs in the liver (Robinson et al., 1991; Pace
et al., 1991). Most of the available studies show minimal if any catabolism (process of breaking
down molecules into smaller units to release energy). Microcystins can be conjugated with
cysteine and glutathione to increase their solubility and facilitate excretion (Kondo et al., 1996).
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However, it is not clear whether hepatic cytochromes, such as cytochrome P450-facilitated
oxidation, precedes conjugation (Cote et al., 1986; Brooks and Codd, 1987). Both in vivo and in
vitro studies have shown biliary excretion (Falconer et al., 1986; Pace et al., 1991; Robinson et
al., 1991).
2.5.2  Noncancer Health Effects Data

 2.5.2.1   Human Studies

       The human data on the oral toxicity of microcystin-LR are limited by the potential co-
exposure to other pathogens and toxins, by the lack of quantitative information, and by the failure
to control for confounding factors.

       Only a few epidemiological and case studies are available on the toxicity of microcystins
in humans. An outbreak among army recruits who had consumed reservoir water with a
cyanobacteria bloom withM aeruginosa reported symptoms of headache, sore throat, vomiting
and nausea, stomach pain, dry cough, diarrhea, blistering around the mouth, and pneumonia
(Turner et al., 1990). Microcystins, including microcystin-LR, were present in bloom samples.
However, high levels of Escherichia coli were also found in reservoir water after two weeks. The
authors suggested that exposure to microcystins may have had a role in some of the clinical
symptoms.

       An epidemiology study done in Australia compared the hepatic enzyme levels from
patients served by a public water supply contaminated with aM aeruginosa bloom with enzyme
levels from patients living in areas served by water supplies uncontaminated by cyanobacteria
(Falconer et al., 1983). Although the authors observed significant variability in enzyme levels
between the two groups, the findings were attributed by the authors  to the imprecise method of
study participant selection and confounding factors such as alcoholism and chronic kidney disease
among some  of the participants.

       A cross-sectional study done in China assessed the relationship between the consumption
of water and food (carp and duck) contaminated with microcystins and liver damage in children
(Li et al., 201 la). The authors found that mean serum levels of microcystins ranged from below
detection to 1.3 ug microcystin-LR equivalents/L. According to the  authors, hepatitis B infection
was a greater risk for liver damage among these children than the microcystin exposure.

       Acute intoxication with microcystin-producing cyanobacteria blooms in recreational water
was reported  in Argentina in  2007 (Giannuzzi et al., 2011). A single person was immersed in a
Microcystis bloom with concentrations of 48.6 |ig/L. After four hours of exposure, the patient
exhibited fever, nausea, and abdominal pain, and three days later, presented dyspnea and
respiratory distress and was diagnosed with an atypical pneumonia.  A week after the exposure,
the patient developed a hepatotoxicosis with a significant increase of alanine aminotransferase
(ALT), aspartate aminotransferase (AST) and y-glutamyltransferase (yGT).  The patient
completely recovered within  20 days.
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       An outbreak of acute liver failure occurred in a dialysis clinic in 1996 in Caruaru, Brazil
where dialysis water was contaminated with microcystins, and possibly cylindrospermopsin. Of
the 130 patients who received their routine hemodialysis treatment (intravenously) at that time,
116 reported symptoms of headache, eye pain, blurred vision, nausea and vomiting. Subsequently,
100 of the affected patients developed acute liver failure and, of these, 76 died (Carmichael et al.,
2001; Jochimsen et al., 1998). Analyses of blood, sera, and liver samples from the patients
revealed microcystins. Although the patients in the study had pre-existing diseases, the direct
intravenous  exposure to dialysate prepared from surface drinking water supplies put them at risk
for cyanotoxin exposure and resultant adverse effects (Hilborn et al., 2013).

       In another contamination event at a dialysis center in Rio de Janeiro, Brazil in 2001, 44
dialysis patients were potentially exposed to microcystin concentrations of 0.32 |ig/L, detected in
the activated carbon filter used in an intermediate step for treating drinking water to prepare
dialysate (Scares et al., 2005). Concentrations of 0.4 jig/L microcystin-LR were detected in the
drinking water. Serum samples were collected from 13 dialysis patients 31 to 38 days after the
detections in water samples, and patients were monitored for eight weeks. Concentrations of
microcystin-LR in the serum ranged from 0.46 to 0.96 ng/mL. Although the biochemical
outcomes varied among the patients, markers of hepatic cellular injury chlolestasis (elevations of
AST, ALT bilirubin, ALP and GOT) in serum during weeks one to eight after treatment
frequently exceeded normal values. Since microcystin-LR was not detected during weekly
monitoring after the first detection, the authors suggested that the patients were not continuously
exposed to the toxin and that the toxin detected in the serum after eight weeks may have been
present in the form of bound toxin in the liver (Scares et al., 2005). Results were consistent with a
mild to moderate mixed liver injury.
2.5.2.2  Animal Studies

       Most of the information on the noncancer effects of microcystins in animals is from oral
and intraperitoneal (i.p.) administration studies in mice and rats exposed to purified microcystin-
LR. Liver effects are observed following acute oral exposure to microcystin-LR (Yoshida et al.,
1997; Ito et al., 1997b; Fawell et al., 1999). Effects on the liver, kidney, and male reproductive
system (testicular function and sperm quality), including changes in organ weights and
histopathological lesions, are observed following short-term and subchronic oral exposure to
microcystin-LR (Heinze, 1999; Fawell et al., 1999; Huang et al., 2011; Chen et al., 2011). Oral
and i.p. developmental toxicity studies in mice provide some evidence for fetal body weight
changes and maternal mortality (Fawell et al., 1999; Chernoff et al., 2002).

       According to the authors, no clinical signs of toxicity were observed in a chronic study
done in mice for 18 months by Ueno et al. (1999). Although histopathology from a 280  day study
in mice revealed infiltrating lymphocytes and fatty degeneration in the livers, no quantitative data
were provided in the study (Zhang et al., 2012).
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2.5.3       Mode of Action for Noncancer Health Effects

       Mechanistic studies have shown the importance of membrane transporters for systemic
uptake and tissue distribution of microcystin by all exposure routes (Fischer et al. 2005; Feurstein
et al., 2010). The importance of the membrane transporters to tissue access is demonstrated when
a reduction in, or lack of, liver damage happens following OATp inhibition (Hermansky et al.,
1990 a,b; Thompson and Pace,  1992).

       The uptake of microcystins causes protein phosphatase inhibition and a loss of
coordination between kinase phosphorylation and phosphatase dephosphorylation, which results
in the destabilization of the cytoskeleton. This event initiates altered  cell function followed by
cellular apoptosis and necrosis (Barford et al.,  1998). Both cellular kinases and phosphatases keep
the balance between phosphorylation and dephosphorylation of key cellular proteins controlling
metabolic processes, gene regulation, cell cycle control, transport and secretory processes,
organization of the cytoskeleton and cell adhesion. Each of the microcystin congeners evaluated
(LR, LA, and LL) interacts with catalytic subunits of protein phosphatases PP1 and PP2A,
inhibiting their functions (Craig et al., 1996).

       As a consequence of the microcystin-induced changes in cytoskeleton, increases in
apoptosis and reactive oxygen species (ROS) occur. In both in vitro and in vivo studies, cellular
pro-apoptotic Bax and Bid proteins increased while anti-apoptotic Bcl-2 decreased (Fu et al.,
2005; Weng et al., 2007; Xing et al., 2008; Takumi et al., 2010; Huang et al., 2011; Li et al.,
201 Ib). Mitochondrial membrane potential and permeability transition pore changes (Ding and
Ong, 2003; Zhou et al., 2012) lead to membrane loss of cytochrome c, a biomarker for apoptotic
events. Wei et al., (2008) found a time-dependent increase in ROS production and lipid
peroxidation in mice after exposure to microcystin-LR. After receiving a 55 |ig/kg of body weight
i.p. injection of microcystin-LR, the levels of hepatic ROS increased rapidly within 0.5 hours and
continued to accumulate for up to 12 hours in a time-dependent manner.
2.5.4       Carcinogenicity Data

       Several human epidemiological studies from China have reported an association between
liver or colon cancer and consumption of drinking water from surface waters containing
cyanobacteria and microcystins (Ueno et al., 1996; Zhou et al., 2002). In these studies, a
concentrations measured in a surface drinking water supply were used as a surrogate for exposure
to microcystins. Individual exposure to microcystins was not estimated, and there was no
examination of numerous possible confounding factors, such as co-occurring chemical
contaminants or hepatitis infections in the population.

       A study done by Flemming et  al. (2002, 2004) in Florida failed to find a significant
association for primary liver cancer between populations living in areas receiving their drinking
water from a surface water treatment plant (with the potential for microcystin exposures), and the
Florida general population, or those receiving their water from ground-water sources. The one
significant association observed was between those people in the surface water service areas,
versus those in their surrounding areas described as buffer zones. However, the nature of the
water supply for the buffer zones were not identified.
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       The only longer-term oral animal study of purified microcystin-LR was conducted by Ito
et al. (1997b). Ito et al. (1997b) administered 80 jig microcystin-LR/kg/day by gavage to mice for
80 or 100 days over 28 weeks (7 months). This single dose failed to induce neoplastic nodules of
the liver. The lack of hyperplastic nodules at 7 months suggests that microcystins are not a
mutagenic initiator of tumors, however, the fairly short duration may have been a limiting factor.

       Several studies suggest that microcystin-LR is a tumor promoter. In these studies, animals
were first exposed to substances known to be tumor initiators (e.g. N-methyl-N-nitroso urea or
NDEA) alone, or in combination with microcystin-LR at i.p. doses known to have no significant
impact on liver weight. The combination of the initiator and the microcystin-LR significantly
increased the number and area of glutathione ^-transferase placental form-positive (GST-P) foci
when compared to treatment with the initiator alone. The same was true for situations where the
initiator treatment was combined with a partial hepatectomy (to stimulate tissue repair) and then
exposed to microcystins i.p. (Nishiwaki-Matsushima et al., 1992; Ohta et al., 1994). GST-P foci
are regarded as indicators for potential tumors formation.  The results from these studies support
the classification of microcystin as a tumor promoter.
2.6     Conceptual Model for Microcystins

       The conceptual model is intended to explore potential links of exposure to a contaminant
or stressor with the adverse effects and toxicological endpoints important for management goals,
including the development of HA values. The conceptual model demonstrates the relationship
between exposure to microcystins in drinking water and adverse health effects in the populations
at risk.

       HAs describe non-regulatory concentrations of drinking water contaminants at which
adverse health effects are not anticipated to occur over specific exposure durations (e.g., one-day,
ten-days, and a lifetime). HAs also contain a margin of safety to protect sensitive members of the
population. They serve as informal technical guidance to assist federal, state and local officials, as
well as managers of public or community water systems, in protecting public health. They are not
to be construed as legally enforceable federal standards.

       Assessment endpoints for HAs can be developed for both short-term (one-day and ten-
day) and lifetime exposure periods using information on the non-carcinogenic and carcinogenic
toxicological endpoints of concern. Where data are available, endpoints will reflect susceptible
and/or more highly exposed populations.

    •  A One-day HA is typically calculated for an infant (0-12 months or 10kg child), assuming
       a single acute exposure to the chemical and is generally derived from a study of less than
       seven days' duration.

    •  A Ten-day HA is typically calculated for an infant (0-12 months or 10kg child), assuming
       a limited period of exposure of one to two weeks, and is generally derived from a study of
       7 to 30-days duration.
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   •   A Lifetime HA is derived for an adult (>21 years or 80kg adult), and assumes an exposure
       period over a lifetime (approximately 70 years). It is usually derived from a chronic study
       of two years duration, but subchronic studies may be used by adjusting the uncertainty
       factor employed in the calculation. For carcinogens, the HA documents typically provide
       the concentrations in drinking water associated with risks for one excess cancer case per
       ten thousand persons exposed up to one excess cancer case per million exposed for Group
       A and B carcinogens and those classified as known or likely carcinogens (U.S. EPA,
       1986, 2005). Cancer risks are not provided for Group C carcinogens or those classified as
       "suggestive", unless the cancer risk has been quantified.

       For each assessment endpoint EPA uses one or more measures of effect (also referred to
as a point of departure), which describe the change in the attribute of the assessment endpoint in
response to chemical exposure, to develop acute, short-term, longer term (subchronic) or chronic
reference values when the data are available. The measures of effect selected represent impacts on
survival, growth, system function, reproduction and development.

       This conceptual model provides useful information to characterize and communicate the
potential health risks related to exposure to cyanotoxins in drinking water. The sources of
cyanotoxins in drinking water, the route of exposure for biological receptors of concern (e.g., via
various human activities such as drinking, food preparation and consumption) and the potential
assessment endpoints (i.e., effects such as kidney and liver toxicity, and reproductive and
developmental effects) due to exposure to microcystins are depicted in the conceptual diagram
below (Figure 2-3).
2.6.1       Conceptual Model Diagram

       Cyanobacteria are a common part of freshwater and marine ecosystems. An increase in
water column stability, high water temperatures, elevated concentrations of nutrients, and low
light intensity have been associated with an increase and or dominance of microcystin-producing
cyanobacteria in surface waters (or aquatic ecosystems).  The presence of detectable
concentrations of cyanotoxins in the environment is closely associated with these blooms. Winds
and water currents can potentially transport cyanobacterial blooms to areas within the proximity
of water intakes for drinking water treatment plants. If not managed in source waters, or removed
during drinking water treatment, cyanobacteria and cyanotoxins may result in exposure that could
potentially affect human health.
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Figure 2-3. Conceptual Model of Exposure Pathways to Microcystins in Drinking Water
STRESSOR
SOURCES
EXPOSURE ROUTE
RECEPTORS
                                          Microcystins
                            Lakes. Reservoirs and Rivers
Shallow ground water under the
direct influence of surface water
                                          Finished Drinking Water

Oral



-

Drinking
water

Cooking with
water

Incidental
ingestion while
showering



Incidental ingestion
while outside activities
(gardening, car
washing, etc.)

Dermal



Inhalation

Showering/
Bathing
Incidental
— i inhalation while
showering

Washing
dishes

Outside
activities
(gardening, car
washing, etc.)

Incidental
— inhalation while
washing dishes

Intravenous
1
' 	 Dialysis

EXDPOINTS
Liver
Damage

Kidney
Damage
Reproductive
Effects
Developmental
Effects
Cancer
Quantitative
Data Available

Incomplete or
Quantitative Data
Not Available
             Drinking Water Health Advisory for Microcystins-June 2015
                             21

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2.6.2      Factors Considered in the Conceptual Model for Microcystins

Stressors: For this HA, the stressor is microcystins concentrations in finished drinking water.

Sources: Sources of microcystins include potential sources of drinking water such as rivers,
reservoirs, and lakes in the U.S. where blooms producing microcystins occur. Shallow private
wells under the direct influence of surface water (in hydraulic connection to a surface water body)
can also be impacted by microcystins-producing blooms, if the toxins are drawn into the well
along with the water from the surface water. There is substantially less information on exposure
from this source.

Routes of exposure: Exposure to cyanotoxins from contaminated drinking water sources may
occur via oral exposure (drinking water, cooking with water, and incidental ingesting from
showering); dermal exposure (contact of exposed parts of the body during bathing or showering,
washing dishes, or outside activities); inhalation exposure (during bathing, showering or washing
dishes,); or intravenous exposure (e.g. via dialysis). Toxicity data are available for the oral route
of exposure from drinking water, but are not available to quantify dose response for other
exposure routes (inhalation, dermal, dietary, and intravenous exposures).

Receptors: The general population  (adults and children) could be exposed to cyanotoxins through
dermal contact, inhalation and/or ingestion. Infants and pre-school age children can be at greater
risk to microcystins because they consume more water per body weight than do adults. Other
individuals of potential sensitivity are persons with kidney and/or liver disease due to the
compromised detoxification mechanisms in the liver and impaired excretory mechanisms in  the
kidney.  There are no human data to quantify risk to pregnant woman or to evaluate the transfer of
cyanotoxins across the placenta. Data are also not available on the transfer of cyanotoxins through
the milk from nursing mothers or regarding the risk to the elderly. Given this lack of information,
pregnant women, nursing mothers,  and the elderly may also be potentially sensitive populations.
Data from the episode in a dialysis  clinic in Caruaru, Brazil where microcystins were not removed
by treatment of dialysis water,  identify dialysis patients as a population of potential concern  in
cases where the drinking water source for the clinic is contaminated with cyanotoxins. Data  are
not available to derive a One-day HA for children because studies with single oral dosing do not
provide dose-response information. A lifetime HA for microcystins is not recommended as the
types of exposures being considered are short-term and episodic in nature. Although the majority
of the cyanobacterial blooms in the U.S. occur seasonally, usually during late summer, some
toxin-producing strains can occur early in the season and can last for days or weeks.

Endpoints: Human data on oral toxicity of microcystins are limited, but suggest the liver as the
primary target organ. Acute, short-term, and subchronic studies in animals also demonstrate  that
the liver and kidney are target organs. In addition, some studies suggest that microcystins may
lead to reproductive and developmental effects. Studies have suggested that microcystins have
tumor promotion potential if there has been co-exposure to a carcinogen or cellular organ damage.
However, these data are limited, and there has been no long term bioassay in animals to evaluate
cancer. Available toxicity data are described in the Health Effects Support Document  (HESD)for
Microcystins (U.S. EPA, 2015a), and indicate that the primary target organ for microcystins  is the
liver. Kidney and reproductive effects in male mice were also observed, but were either not as
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sensitive as the liver or lack confirmation from more than one laboratory. Data are inadequate to
assess the carcinogenic potential of microcystins at this time.
2.7     Analysis Plan

       The Health Effects Support Documentfor Microcystins (HESD, U.S. EPA, 2015 a),
provides the health effects basis for development of the HA, including the science-based
decisions providing the basis for estimating the point of departure. To develop the HESD for
microcystins, a comprehensive literature search was conducted from January 2013 to May 2014
using Toxicology Literature Online (TOXLINE), PubMed component, and Google Scholar to
ensure the most recent published information on microcystins was included. Some of the  search
terms included in the literature search were microcystin, microcystin congeners, human toxicity,
animal toxicity, in vitro toxicity, in vivo toxicity, occurrence, environmental fate,  mobility, and
persistence. EPA assembled available information on occurrence, environmental fate,
mechanisms of toxicity, acute, short-term, subchronic and chronic toxicity and cancer in humans
and animals, toxicokinetics, and exposure. Additionally, EPA considered information from the
following risk assessments during the development of the microcystins health risk assessment:

   •   Health Canada (2012) Toxicity Profile for Cyanobacterial Toxins

   •   Enzo Funari and Emanuela Testai (2008) Human Health Risk Assessment Related to
       Cyanotoxins Exposure

   •   Tai Nguyen Duy, Paul Lam, Glen Shaw and Des Connell (2000) Toxicology and Risk
       Assessment of Freshwater Cyanobacterial  (Blue-Green Algal) Toxins in Water

       The toxicity data available for an individual pollutant vary significantly. An evaluation of
available data was performed by EPA to determine data acceptability. The following study quality
considerations from U.S. EPA's (2002) A Review of the Reference Dose and Reference
Concentration Processes were used in selection of the  studies for inclusion in the HESD and
development of the HA.

   •   Clearly defined and stated hypothesis.

   •   Adequate description of the  study protocol, methods, and statistical analyses.

   •   Evaluation of appropriate endpoints. Toxicity depends on the amount, duration, timing,
       and pattern of exposure and  may range from frank effects (e.g., mortality) to more subtle
       biochemical, physiological, pathological, or functional changes in multiple organs and
       tissues.

   •   Application of the appropriate statistical procedures to determine an effect.

   •   Establishment of dose-response relationship (i.e.,  no observed adverse effect level
       (NOAEL) and/or lowest observed adverse  effect level (LOAEL) or data amenable to
       modeling of the dose-response in order to identify a point of departure for a change in the
       effect considered to be adverse (out of the range of normal biological viability). The
       NOAEL is the highest exposure level at which there are no biologically significant
                Drinking Water Health Advisory for Microcystins-June 2015            23

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       increases in the frequency or severity of adverse effect between the exposed population
       and its appropriate control. The LOAEL is the lowest exposure level at which there are
       biologically significant increases in frequency or severity of adverse effects between the
       exposed population and its appropriate control group.

       After the available studies were evaluated for inclusion in the HESD and HA, the critical
study was selected based on consideration of factors including exposure duration (comparable to
the duration of the HA being derived), route of exposure (oral exposure via drinking water,
gavage, or diet is preferred), species sensitivity, comparison of the point of departure with other
available studies demonstrating an effect, and confidence in the study (U.S. EPA, 1999). Once, a
point of departure is chosen for quantification, uncertainty factors appropriate for the study
selected are then applied to the point of departure to account for variability and uncertainty in the
available data.

       For microcystins, toxicity and exposure data are available to develop a Ten-day HA. EPA
used measures of effect and estimates of exposure to derive the Ten-day HAs using the following
equation:
                     HA  =
NOAEL or LOAEL or BMDL
         UF x DWI/BW
Where:
  NOAEL or  = No- or Lowest-Observed-Adverse-Effect Level (mg/kg bw/day) from a study
    LOAEL    of an appropriate duration (7 to 30 days).

     BMDL  = When the data available are adequate, benchmark dose (BMD) modeling can
                be performed to determine the point of departure for the calculation of HAs.
                The benchmark dose approach involves dose-response modeling to obtain
                dose levels corresponding to a specific response level near the low end of the
                observable range of the data (U.S.EPA, 2012). The lower 95% confidence
                limit is termed the benchmark dose level (BMDL).

         UF  = Uncertainty factors (UF) account for: (1) intraspecies variability (variation in
                susceptibility across individuals); (2) interspecies variability (uncertainty in
                extrapolating animal  data to humans; (3) uncertainty in extrapolating from a
                LOAEL to a NOAEL; and (4) uncertainty associated with extrapolation when
                the database is incomplete. These are described in U.S. EPA, 1999 and U.S.
                EPA, 2002.

   DWI/BW  = For children, a normalized ratio of drinking water ingestion to body weight
                (DWI/BW) was calculated using data for infants  (birth to <12 months). The
                estimated drinking water intake body weight ratio (L/kg/day) used for birth to
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                                                     24

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 <12 months of age are the 90th percentile values of the consumers only
 estimates of direct and indirect water ingestion based on 1994-1996, 1998
 CSFII (Continuing Survey of Food Intakes by Individuals) (community water,
 mL/kg/day) in Table 3-19 in the U.S. EPA (201 la) Exposure Factors
 Handbook. The time weighted average of DWI/BW ratios values was derived
 from multiplication of age-specific DWI/BW ratios  (birth to <1 month, 1 to
 <3 months, 3 to <6 months,  and 6 to <12 months) by the age-specific fraction
 of infant exposures for these time periods.

 For adults (>21 years of age), EPA updated the default BW assumption to 80
 kg based on National Health and Nutrition Examination Survey (NHANES)
 data from 1999 to 2006 as reported in Table 8.1 of EPA's Exposure Factors
 Handbook (U.S. EPA, 201 la). The updated BW represents the mean weight
 for adults ages 21 and older.

 EPA updated the default DWI to 2.5 L/d, rounded from 2.546 L/d, based on
 NHANES data from 2003 to 2006 as reported in EPA's Exposure Factors
 Handbook (U.S. EPA 201 la, Table 3-33). This rate  represents the consumer's
 only estimate of combined direct and indirect community water ingestion at
 the 90th percentile for adults ages 21 and older.
Drinking Water Health Advisory for Microcystins-June 2015           25

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3.0 HEALTH EFFECTS ASSESSMENT

       The health effects assessment provides the characterization of adverse effects and includes
the hazard identification and dose-response assessment. The hazard identification includes
consideration of available information on toxicokinetics; identification, synthesis and evaluation
of studies describing the health effects of microcystins; and the potential modes of action
(MOAs), or toxicity pathways related to the health effects identified.
3.1     Dose-Response

3.1.1       Study Selection

       The critical study chosen for determining the guideline value is a short-term study by
Heinze (1999) in which 11-week-old male hybrid rats (Fl generation of female WELS/Fohm x
male BDIX) were administered microcystin-LR via drinking water for 28 days at concentrations
of 0 (n=10), 50 (n=10) or  150 (n=10) ug/kg body weight (Heinze,  1999). Water consumption was
measured daily, and rats were weighed at weekly intervals. The dose estimates provided by the
authors were not adjusted to account for incomplete drinking water consumption (3-7% of
supplied water was not consumed over the 28-day period). Rats were sacrificed by exsanguination
under ether anesthesia after 28 days of exposure, and evaluation of hematology, serum
biochemistry plus histopathology of liver and kidneys, and measurement of organ  weights (liver,
kidneys, adrenals, spleen and thymus) was performed.

       Hematological evaluation showed an increase of 38% in the number of leukocytes at the
highest dose group (150 ug/kg body weight). Serum biochemistry  showed a significant increase in
both treatment groups in mean levels of alkaline phosphatase (ALP)  and lactate dehydrogenase
(LDH); 84 and 100% increase in LDH, and 34 and 33% increase in ALP, in the low and high dose
groups respectively. No changes were observed in mean levels of AST (aspartate
aminotransferase), and ALT (alanine aminotransferase). An increase in relative liver weights was
observed in a dose-dependent manner; 17% at 50 ug/kg body weight, and 26% at 150 ug/kg body
weight. Mean enzyme levels and relative liver weights are shown in Table 3-1.

       A dose-dependent increase in absolute liver weight was also reported, and  data on the liver
weights were provided by the author in a personal communication. A dose-dependent increase in
the average absolute liver weights was also observed in all groups: 8.8 grams at the control group,
9.70 grams at the lower dose and 10.51 grams at the high dose (Table 3-1). No statistically
significant changes in other organ weights or body weights were reported, and no effects on the
kidneys were observed. Table 3-2 summarizes the histological observations of liver lesions. Liver
lesions were considered toxic and spread diffusely throughout the parenchyma indicating cell
damage expressed by an increase in cell volume, an increase in mitochondria, cell  necrosis, the
activation of Kupffer cells, and an increase in the amounts of periodic acid-Schiff  (PAS)-positive
substances. Liver lesions were observed in both treatment groups. No kidney effects were
observed in either dose groups.  The LOAEL was determined to be 50 ug/kg/day. The selection of
Heinze (1999) as the critical study was based on the appropriateness of the study duration, the use
               Drinking Water Health Advisory for Microcystins-June 2015            26

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Table 3-1. Liver Weights and Serum Enzyme Levels in Rats Ingesting Microcystin-LR in
Drinking Water (Heinze, 1999)

Control
(Mean ± SD)
50 ug/kg
(Mean ± SD)
150 ug/kg
(Mean ± SD)
Serum Enzymes
Alkaline phosphatase (ALP)
(microkatals/L)
Lactate dehydrogenase (LDH)
(microkatals/L)
9.67 ±2.20
16.64 ±4.48
13.00±3.81*
30.64 ±5. 05*
12.86 ± 1.85*
33.58± 1.16*
Liver Weight
Relative (g/100 g body weight)
Absolute (g)**
2.75 ± 0.29
8.28 ± 1.37
3.22 ±0.34*
9.70 ± 1.32
3.47 ±0.49*
10.51 ± 1.02
       * p<0.05 when compared with control; katal=conversion rate of 1 mole of substrate per second.
       * information provided by the author through a personal communication.
Table 3-2. Histological Evaluation of the Rat Livers after Ingesting Microcystin-LR in
Drinking Water (Heinze, 1999)
•
Activation of
Kupffer Cells
Degenerative
and Necrotic
Hepatocytes
with
Hemorrhage
Degenerative
and Necrotic
Hepatocytes
without
Hemorrhage
PAS-positive
Material
Control
Slight
Moderate
Intensive damage
0
0
0
0
0
0
0
0
0
1
0
0
50 jig/kg
Slight
Moderate
Intensive damage
0
10
0
4
6
0
0
0
0
5
5
0
150 ug/kg
Slight
Moderate
Intensive damage
0
10
0
0
6
3
0
1
0
0
8
2
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27

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of multiple doses, dose-related toxicological responses, and histopathological evaluations of
toxicity.


3.1.2       Endpoint Selection

       The point of departure selected from the Heinze (1999) study is the LOAEL (50
ug/kg/day) for liver effects (increased liver weight, slight to moderate liver necrosis lesions, with
or without hemorrhages at the low dose and increased severity at the high dose, and changes in
serum enzymes indicative of liver damage). For the lesions, incidence increases from one animal
impacted in the control group to ten animals impacted in the dosed groups. This dose-response is
more dramatic than the difference in liver weight between the control and low dose (1.17 fold)
and the differences in the ALP and LDH levels between the control and low dose group (1.34 and
1.84-fold, respectively). Therefore, the liver lesions are identified as the endpoint of greatest
concern. These differences also advise against application of benchmark dose modeling for these
effects. The male and female mice in the Fawell et al (1999) study displayed liver lesions, but the
difference between controls and the low dose group (40 ug/kg/day) was less than two-fold.  In an
i.p. infusion study by Guzman and Solter (1999) with a more direct delivery of dose to the liver,
necrosis was observed at doses of 32 and 48 ug/kg/day, but not at a dose of 16 ug/kg/day, thus
providing support for the critical effect and dose.
3.2     Ten-day Health Advisory

       This Ten-day HA is applied to total microcystins using microcystin-LR as a surrogate.
The Ten-day HA is considered protective of non-carcinogenic adverse health effects over a ten-
day exposure to microcystins in drinking water.

3.2.1  Bottle-fed Infants and Young Children of Pre-school Age

The Ten-day HA for bottle-fed infants and young children of pre-school age is calculated as
follows:
                   „     ,   TTA         50 jug/kg/day
                   Ten-day HA =	^    —	 =0.3 ug/L
                                    1000 x 0.15L/kg/day
Where:
         50 ug/kg/day     =  The LOAEL for liver effects in 11-week-old male hybrid rats
                             exposed to microcystin-LR in drinking water for 28 days
                             (Heinze, 1999).
         1000            =  The composite UF including a 10 for intraspecies variability
                             (UFn), a 10 for interspecies differences (UFA), a 3 for LOAEL to
                             NOAEL extrapolation (UFi,), and a 3 for uncertainties in the
                             database (UFo).
         0.15 L/kg/day    =  Normalized drinking water intake per unit body weight over the
                             first year of life based on the 90th percentile of drinking water
                             consumption and the mean body weight (U.S. EPA, 201 la).
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The Ten-day HA of 0.3 |ig/L is considered protective of non-carcinogenic adverse health effects
for bottle-fed infants and young children of pre-school age over a ten-day exposure to
microcystins in drinking water.
3.2.2       School-age Children through Adults

The Ten-day HA for school-age children through adults is calculated as follows:
                T    A    UA          50
                Ten-day HA  = -      — - - =1.6 ug/L
                                  1000  x 0.03 L/kg/day
         50 |ig/kg/day   =   The LOAEL for liver effects in 1 1 -week-old male hybrid
                            rats exposed to microcystin-LR in drinking water for 28
                            days (Heinze, 1999).
         1000           =   The composite UF including a 10 for intraspecies
                            variability (UFn), a 10 for interspecies differences (UFA), a
                            3 for LOAEL to NOAEL extrapolation (UFi,), and a 3 for
                            uncertainties in the database (UFo).
         0.03 L/kg/day   =   Drinking water intake per unit body weight based on adult
                            default values of 2.5 L/day and 80 kg (U.S. EPA, 201 la).

The Ten-day HA of 1.6 jig/L is considered protective of non-carcinogenic adverse health effects
for children of school age through adults over a ten-day exposure to microcystins in drinking
water.
3.2.3       Uncertainty Factor Application

   •   UFn - A Ten-fold value is applied to account for variability in the human population. No
       information was available to characterize interindividual and age-related variability in the
       toxicokinetics or toxicodynamics among humans. Individuals with pre-existing liver
       problems could be more sensitive to microcystins exposures than the general population.
       Pregnant woman, nursing mothers, and the elderly could also be sensitive to microcystins
       exposures.

   •   UFA - A Ten-fold value is applied to account for uncertainty in extrapolating from
       laboratory animals to humans (i.e., interspecies variability). Information to quantitatively
       assess toxicokinetic or toxicodynamic differences between animals and humans is
       unavailable for microcystins. Allometric scaling is not applied in the development of the
       Ten-day HA values for microcystins. The allometric scaling approach is derived from the
       relationship between body surface area and basal metabolic rate in adults (U.S. EPA,
       201 Ib). This approach is not appropriate for infants and children due to the comparatively
       slower clearance during these ages and the limited toxicokinetic data available to assess
       the appropriateness of body weight scaling in early life.
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           - An uncertainty factor of 3 (10°5 = 3.16) is selected to account for the extrapolation
       from a LOAEL to a NOAEL. The threefold factor is justified based on the evidence
       suggesting that the uptake of microcystins by tissues requires membrane transporters.
       Uptake from the intestines involves both apical and basolateral transporters, uptake by the
       microvilli capillaries and portal transport to the liver. Transporters are again necessary for
       hepatic uptake. When there is slow infusion into the peritoneum and into the portal
       intraperitoneal capillaries, uptake is described as rapid because of the rich blood supply
       and large surface area of the  peritoneal cavity (Klassen, 1996). Delivery of the
       microcystins to the intraperitoneum increases the amount of the dose that reaches the liver
       for three additional reasons:  1) the apical and basolateral intestinal barriers to uptake are
       eliminated with the i.p. infusion; 2) there is no dilution of dose by the gastric plus
       intestinal fluids as when food residues are in the gastrointestinal track; and 3) there is no
       delay in reaching the site of absorption because of gastric emptying time (Klassen, 1996).
       In addition, facilitated transporter kinetics are similar to Michaelis Menton enzyme
       kinetics in that there are Km  and Vmax components that are defined by the affinity of the
       transported substance for the transporter.

       In the Guzman and Solter (1999) intraperitoneal infusion study in rats, the NOAEL is 16
       |ig/kg/day and the LOAEL is 32 jig/kg/day, a two-fold difference.  There is no reason to
       believe that the less direct delivery from the intestines to the liver following oral
       exposures through drinking water (as was used in Heinze, 1999) would have a more than
       3-fold separation between a NOAEL and LOAEL had there been one in the Heinze (1999)
       study.

    •   UFo - An uncertainty factor of 3 (1005 = 3.16) is selected to account for deficiencies in the
       database for microcystins. The database includes limited human data, including studies
       evaluating the association between microcystin exposure and cancers in liver and colon,
       and systemic effects including liver endpoints such as elevated liver enzymes. Oral and
       i.p. acute and short-term studies on mice and rats, and subchronic studies done in mice are
       available.  Chronic data are also available for microcystin, however, are limited by the lack
       of quantitative data provided in the study. Additionally, there are limited neurotoxicity
       studies (including a recent publication on developmental neurotoxicity) and several i.p.
       reproductive and developmental toxicity studies. The database lacks a multi-generation
       reproductive toxicity study.

    The default factors typically used cover  a single order of magnitude (i.e., 101). By convention,
in the Agency, a value of 3 is used in place of one-half power (i.e., 101/2) when appropriate (U.S.
EPA, 2002).
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4.0 RISK CHARACTERIZATION

     The following topics describe important conclusions used in the derivation of the health
advisory. This section characterizes each topic and its impact on the health advisory.

4.1     Use of microcystin-LR as a surrogate for total microcystins

       Among the approximately 100 different congeners of microcystins known to exist,
microcystin-LR is the most common. The difference in toxicity of microcystin congeners depends
on the amino acid composition (Falconer, 2005). Stoner et al. (1989) administered by
intraperitoneal (i.p.) purified microcystin congeners (-LR, -LA, -LY and -RR) into ten or more
adult male and female Swiss albino mice. Necropsies were performed to confirm the presence of
the pathognomonic hemorrhagic livers. The authors reported 50% lethal doses (LDso) of 36 ng/g-
bw for -LR, 39 ng/g-bw for -LA, 91 ng/g- bw for -LY and 111 ng/g-bw for -RR. Similarly, Gupta
et al., (2003) determined LDso for the microcystin congeners LR, RR and YR in female mice
using DNA fragmentation assay and histopathology examinations of the liver and lung.  The acute
LDso determination showed that the most toxic congener was microcystin-LR (43.0 |ig/kg),
followed by microcystin-YR (110.6 |ig/kg) and microcystin-RR (235.4 jig/kg).  The most toxic
microcystins are those with the more hydrophobic L-amino acids (-LA, -LR, -and -YM), and the
least toxic are those with hydrophilic amino acids, such as microcystin-RR.

       Wolf and Frank (2002) proposed toxicity equivalency factors (TEFs) for the four major
microcystin congeners based on LDso values obtained after i.p. administration. The proposed
TEFs, using microcystin-LR as the index compound (TEF=1.0) were 1.0 for microcystin-LA and
microcystin-YR and 0.1 for microcystin-RR. The application of TEFs based on i.p. LDso values to
assessment of risk from oral or dermal exposure is questionable given that differences in
lipophilicity and polarity of the congeners may lead to variable absorption by non-injection routes
of exposure.

       The potential health risks from exposure to mixtures of microcystin congeners is
unknown, and since microcystin-LR is one of the most potent congeners and has the majority of
toxicological data on adverse health effects, microcystin-LR is used as a surrogate for all
microcystins in the health advisory.
4.2     Consideration of Study Duration

       EPA used a 28-day study conducted by Heinze (1999) to derive the Ten-day HA for
microcystins. It is standard to use studies that are 7 to 30 days in duration to derive a 10-day
advisory value. In the study conducted by Heinze (1999), rats were dosed daily via drinking water
with microcystin and sacrificed at the conclusion of the study. No interim sacrifices were
performed to evaluate effects at 10 days or any other time less than the full 28 days. At the
conclusion of the 28-day study, adverse effects observed in the liver included increases in liver
weight, slight to moderate liver necrosis lesions accompanying hemorrhages at the low dose with
increased severity at the high dose, and changes in serum enzymes indicative of liver damage.
Given the lack of interim effects data, it is not known when during the 28-day study these effects
were manifested.
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4.3     Consideration of Reproductive Effects as Endpoint

       Upon consideration of all available studies, liver effects were considered the most
appropriate basis for quantitation as it was a common finding among oral toxicology studies
(Falconer et al., 1994; Fawell et al., 1999; Ito et al., 1997b). However, while the liver is the
primary target of microcystin toxicity, there have been reports of effects of microcystin-LR on the
male reproductive system and sperm development following oral exposures (Chen et al., 2011).

       In a study conducted by Chen et al. (2011), oral exposures to low concentrations of
microcystin-LR for 3 to 6 months showed reproductive toxicity including decreased sperm counts
and sperm motility, as well as an increase in sperm abnormalities, decreased serum testosterone
and increased serum luteinizing hormone (LH) levels. Because these effects were observed at
doses lower (0.79 mg/kg/day) than those observed for liver effects in Heinze (1999), EPA
evaluated Chen et al. (2011) and the lesions  in the testes and effects on sperm motility as the
potential critical study and points of departure for the derivation of the RfD for microcystins.

       The Chen et al., 2011 study has several limitations in the experimental  design and
reporting. There was a lack of data reported  on testis weights and sperm motility. The authors
reported "no significant differences in testis  weights," but no information was provided on the
weights of the testis or whether there was a trend toward decreasing weights that failed to be
statistically significant. Also, no information was given on the methodology used for sperm
motility evaluation. No information was provided on how samples were handled and what
measurements were made to determine the percentage of sperm motility. Although body weight
and amount of water consumed were measured, these data were not presented, and doses to the
animals were not calculated by the study authors. In addition, the purity of microcystin-LR and
the species  and age of the mouse used were not reported. Male sperm characteristics such as
volume, motility, and structure of sperm differ developmentally by age. Therefore, not knowing
the age of the mice in the study introduces uncertainty in the quantification of the reproductive
effects.

       The fixation and staining of the testes used for microscopic examination
(paraformaldehyde in phosphate-buffered saline (PBS) and paraffin), could result in the
generation of artifacts, such as disruption of the testicular tubes. Cytoplasmic shrinkage and
chromatin aggregations were observed in both control and experimental groups. In order to
preserve the micro structure of the testis, dual fixation such as Davidson's or Bouin's fixation
followed by PAS staining should have been  done. In addition, the histopathology analysis of the
testes reported by the authors did not provide sufficient detail to adequately assess the degree of
damage.

       The quality of the medium used for the sperm analysis, and the lack of additional data
from the sperm analysis measurements carried out through the computer-assisted sperm analysis
(CAS A) are additional limitations in experimental design for this study. Very few details of the
serum hormone assay protocol and the quantitative parameters of sperm motility from the CASA
analysis were provided. Therefore, the calculation for the motility of the sperm was unclear and
could not be verified.
                Drinking Water Health Advisory for Microcystins-June 2015            32

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       Based on the limitations in study design, report and methods used by Chen et al. (2011),
EPA concluded that the quantitative data on decreased sperm counts and sperm motility were not
appropriate for determining the point of departure for the derivation of the RfD for microcystin.
4.4     Allometric Scaling Approach

       Allometric scaling was not applied in the development of the short term RfD for
microcystins. In the development of short-term advisory values (One-day and Ten-day),
parameters are used that reflect exposures and effects for infants up to one year of age, rather than
for adults. The body weight scaling approach is derived from the relationship between body
surface area and basal metabolic rate in adults. Infants/children surface area and basal metabolic
rates are very different than adults with a slower metabolic rate. In addition, limited toxicokinetic
data are available to assess the appropriateness of body weight scaling in early life. The body
weight scaling procedure has typically been applied in the derivation of chronic oral RfDs and
cancer assessments, both of which are concerned with lifetime repeated exposure scenarios (U.S.
EPA, 2012). Thus, given the short term duration of the critical study and the development of a
short term RfD for determination of a Ten-day HA value, and the application of the Ten-day HA
to infants and pre-school age children, the application of the body weight scaling procedure is not
appropriate for this scenario.

       In addition, for short-term advisories (one-day and ten-day duration), EPA assumes all
exposure is derived from drinking water and, therefore, no Relative Source Contribution (RSC)
term is applied. For lifetime health advisory values, EPA does include an RSC that reduces the
advisory value to  account for other potential sources.
4.5     Benchmark Dose (BMD) Modeling Analysis

       The data set reported by Heinze (1999) was evaluated for BMD modeling. Heinze (1999)
demonstrated dose-related liver changes and statistically significant effects at the lowest dose (50
Hg/kg/day). Histological changes were also observed in all the animals (ten) in each dose group
(Table 3-2). Although differences in the degree of necrosis were observed with or without
hemorrhage related to dose, all the histological effects including Kupffer cell activation and PAS
staining showed no dose-response since all ten animals at the low and high doses displayed liver
damage associated with each effect. Therefore, the dose-response for the sum of the incidence
categories (slight, moderate, and intensive damage), are not amenable to BMD modeling. As a
result, the LOAEL of 50 jig/kg/day described by Heinze (1999) was used as the POD for
development of the HA.
4.6     Carcinogenicity Evaluation

       While there is evidence of an association between liver and colorectal cancers in humans
and microcystins exposure and some evidence that microcystin-LR is a tumor promoter in
mechanistic studies, there is inadequate information to assess carcinogenic potential of
microcystins in humans (U.S. EPA, 2005). The human studies are limited by lack of exposure
                Drinking Water Health Advisory for Microcystins-June 2015            33

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information and the uncertainty regarding whether or not these studies adequately controlled for
confounding factors such as Hepatitis B infection. No chronic cancer bioassays for microcystins
in animals are available.

       The only oral study that examined the tumorgenicity of microcystin-LR failed to find
preneoplastic nodules in the livers of groups of 22 mice receiving up to 100 doses of 0 or 80
ug/kg/day over 7 months. Some studies suggest that microcystin-LR is a tumor promoter. Given
the potential impact on the cell cytoskeleton, necrotic  effects on liver cell generation of reactive
oxygen species (ROS), and other biochemical changes, this finding is not surprising. The work by
Nishiwaki-Matsushima et al., 1992 that compares glutathione S-transferase placental form-
positive (P-GST) foci from 10 |ig/L microcystin-LR to that from the phenobarbital (0.05% in the
diet) as a positive control suggests that it is at best a weak promoter. The results from the second
part of the same study that compare P-GST foci following initiation with DEN followed by
microcystin-LR (10 |ig/kg), both before and after a partial hepatectomy, support this conclusion.

       The International Agency for Research on Cancer (IARC) classified microcystin-LR as a
Group 2B (possibly carcinogenic to humans) based on the conclusion that there was strong
evidence supporting a plausible tumor promoter mechanism for these liver toxins. U.S. EPA's
Cancer Guidelines (2005) state that the descriptor of "inadequate information to assess
carcinogenic potential" is appropriate when available data are judged inadequate for applying one
of the other descriptors or for situations where there is little or no pertinent information or
conflicting information. The guidelines also state that  (p. 2-52) "Descriptors can be selected for
an agent that has not been tested in a cancer bioassay if sufficient other information, e.g.,
toxicokinetic and mode of action information, is available to make a strong, convincing, and
logical case through scientific inference". In the case of microcystins, the data suggest that
microcystin-LR may be a tumor promoter but not an initiator. Without stronger epidemiology
data and a chronic bioassay of purified microcystin-LR, the data do not support classifying
microcystin-LR as a carcinogen.
4.7     Uncertainty and Variability

       Several uncertainty factors were applied in several areas to account for incomplete
information. Human data on the toxic effects of microcystins are limited. Quantification of the
absorption, distribution, and elimination of microcystins in humans following oral, inhalation or
dermal exposure is not well understood. The clinical significance in humans for biological
changes observed in experimental animals such as decreased sperm count and motility, and
microscopic lesions in the testes needs further analysis. In animal studies with oral exposures to
microcystins, some adverse effects in males such as reduced testosterone levels, as well as
toxicity to the female reproductive tissues and those of offspring have not been fully
characterized. No data are available to quantify the differences between humans and animals for
the critical health endpoints. There is uncertainty regarding susceptibility and variability in the
human population following exposure to microcystins and the relative toxicity of other
microcystins congeners when compared to microcystin-LR. Additional information is needed on
the potential health risks from mixtures  of microcystins with other cyanotoxins, as well as
biological and chemical stressors present in source water and drinking water supplies.
                Drinking Water Health Advisory for Microcystins-June 2015             34

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       In addition, for short-term advisories (One-day and Ten-day duration), EPA assumes all
exposure is derived from drinking water and, therefore, no Relative Source Contribution (RSC)
term is applied. For lifetime health advisory values, EPA does include an RSC that reduces the
advisory value to account for exposure to other potential sources.

4.8     Susceptibility

       Available animal data are not sufficient to determine if there is a definitive difference in
the response of males versus females following oral exposure to microcystins. Fawell et al. (1999)
observed a slight difference between male and female mice in body weight and serum proteins
(ALT and AST), but no sex-related differences in liver pathology.

       Studies in laboratory rodents suggest that the acute effects of microcystin-LR may be
more pronounced in adult or aged animals than in juvenile animals (Adams et al., 1985; Ito et al.,
1997a; Rao et al., 2005). In these studies, young animals showed little or no effect at microcystin-
LR doses found to be lethal to adult animals. Age-dependent differences in toxicity were observed
after both oral and i.p. exposure, suggesting that differences in gastrointestinal uptake were not
entirely responsible for the effect of age. The relevance of these age-related differences to acute
toxicity in humans  is unknown. However, for infants to one-year olds fed exclusively with
powdered formula prepared with tap water, drinking water is the dominant route of exposure to
cyanotoxins. There are significant differences in exposure between these life-stages that impact
risk.

       Based on the available studies in animals, individuals with liver and/or kidney disease
may  be more susceptible than the general population since the detoxification mechanisms in the
liver and impaired excretory mechanisms in the kidney may be compromised. Data from an
episode in a dialysis clinic in Caruaru, Brazil where microcystins were not removed by treatment
of dialysis water, identify dialysis patients as a population of potential concern in cases where the
drinking water source for the clinic used to prepare the dialysate is contaminated with
cyanotoxins. Other potentially sensitive individuals include pregnant woman, nursing mothers,
and the elderly.
4.9     Distribution of Body Weight and Drinking Water Intake by Age

       Both body weight and drinking water intake are distributions that vary with age. EPA has
developed two health advisory values, a Ten-day HA of 0.3 jig/L based on exposure to infants
over the first year of life, and a Ten-day HA of 1.6 |ig/L based on exposure to adults, over 21
years of age. Section 4.10 discusses how EPA recommends application of these values to other
age groups.

       The U.S. EPA (201 la) Exposure Factors Handbook provides values for drinking water
ingestion rate and corresponding body weight.  The estimated 90th percentile of community water
ingestion for the general population (males and females of all ages) has been used as the default
value for water ingestion. EPA plotted the 90th percentile of drinking water intake using Table 3-
19 for ages <3 years, and Table 3-38 for ages >3 years due to sample size in the respective studies.
Age groups <3 months in Table 3-19 were combined due to insufficient sample sizes. Figure 4.1
                Drinking Water Health Advisory for Microcystins-June 2015            35

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         Figure 4-1. 90th Percentile Drinking Water Ingestion Rates by Age Group
                 0.25
     **%
     sS
    •a


    I
     0)
    "3
     o
    I
    £
    _
    _c
    'C
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    —
    -*j
    I
    o
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                         0.23
       Adapted from U.S. EPA 2011 Exposure Factors Handbook (U.S.EPA, 201 la).
represents the 90th percentile drinking water ingestion rates (L/kg/day) for each age group (located
on top of the columns). Bottle-fed ages are shown in red (first three columns on the left).

       Based on the drinking water intake rates for children <12 months (0.15 L/kg-day), the
exposure of children is over 4 times higher than that of adults >21 years old on a body weight
basis (0.034 L/kg-day). Infants from birth to 3 months may be exclusively bottle-fed and
therefore, have a higher ingestion rate. After 3 months of age, typically around 4 to 6 months of
age, other food and liquids are introduced into the infant diet, lowering the ingestion rate of
drinking water. Drinking water contributes the highest risk of the total cyanotoxin intake for
infants to one-year-olds fed exclusively with powdered formula prepared with tap water
containing cyanotoxins At the age of 6, children's intake of drinking water relative to their body
weight is approximately the same as those of an adult (>21 years). Data evaluating the transfer of
microcystins through breast milk are not available for humans.
4.10    Distribution of Potential Health Advisory Values by Age

       Using the ingestion rates for each age-group (from Figure 4-1), EPA estimated Ten-day
HA values for microcystins for each age group (plotted on Figure 4-2) to demonstrate the
variability due to body weight and drinking water intake by age.
                Drinking Water Health Advisory for Microcystins-June 2015
36

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           Figure 4-2. Ten-day Health Advisories for Microcystins by Age Group
     2.3
     2.2
     2.1
      2
     1.9
     1.8
     1.7
DO •*•"»*
JL 1.4
£-1.3
a 1.2
_> 1.1
<   i
« 0.9
3 0.8
= 0.7
  0.6
  0.5
  0.4
  0.3
  0.2
  0.1
    0
                                       School-age children and
                                          adults l.E
            Bottle fed infants up to
           school age children 0.3 ng/L
          birth to  3to<6  6 to < 12  1 to<2  2 to <3   3 to <6 6 to < 11 11 to <16 16 to <1818 to <21  > 21
           <3    months  months   years    years   years    years    years   years    years    years
          months                              Age Range
        EPA decided to apply the Ten-day HA value calculated for infants over the first year of
life (0.3 |ig/L) to all bottle-fed infants and young children of pre-school age because these age
groups have higher intake per body weight relative to adults. As Figure 4.2 demonstrates, when
the Ten-day HA is estimated by age group, the calculated HA value for infants from birth to 3
months old is 0.2 |ig/L, slightly below the infant health advisory value of 0.3 |ig/L. EPA believes
that infants from birth to 3 months old are not at a disproportionate risk at a 0.3  |ig/L advisory
value because a 30-fold safety factor is built into this calculation to account for human variability
and deficiencies in the database. The estimated Ten-day HA values for infants from 3 months old
through pre-school  age groups (less than 6 years old) are at or above the advisory value  of 0.3
|ig/L. Therefore, children within these age groups are adequately protected by the advisory value
for bottle-fed infants and young children of pre-school age. EPA decided to apply the adult Ten-
day HA value of 1.6 |ig/L to school age children (children older than or equal to 6 years) through
adulthood because children's intake of drinking water relative to body weight in this age group is
almost the same as those of an adult (>21 years).
                Drinking Water Health Advisory for Microcystins-June 2015
                                                                                    37

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5.0 ANALYTICAL METHODS

       This Health Advisory (HA) for the Cyanobacterial Microcystin Toxins is applied to total
microcystins which should include all of the measureable microcystin congeners within the
cyanobacterial cells (intracellular) and outside the cell (extracellular).

       Extracellular microcystins (either dissolved in water or bound to other materials) typically
make up less than 30% of the total microcystin concentration in source water (Graham et al.,
2010). Most of the toxin is intracellular, and released into the water when the cells rupture  or die.
Both intracellular and extracellular microcystins may also be present in treated water, depending
on the type of treatment processes in place. Therefore, it is important to note that analysis for
microcystins should account for both intracellular and extracellular toxins in samples when intact
cells may be present. Release of intracellular microcystins is achieved by rupturing or lysing the
cell walls in order to expose the intracellular microcystins.  Cell lysis can be achieved by a variety
of methods including sequential freeze-thawing, freeze drying, and mechanical or sonic
homogenization. Following cell lysis, microcystins may need to be extracted for some analytical
methods. At low concentrations, the  direct determination of microcystins may not be feasible, and
a preconcentration step may be required. Typically samples are filtered and/or centrifuged  after
cell lysis to remove cell fragments and particulates. This may be followed by freeze-drying or
solid-phase extraction (SPE). Typical elution solvents are dilute acid, methanol, acidified
methanol/water mixtures, and butanol/methanol/water mixtures.

       Preconcentration is generally needed when techniques  such as liquid chromatography are
used in order to achieve limits of detection in the low-|ig/L and ng/L range. Extraction efficiency
has been shown to vary depending on the type of solvent, the hydrophobicity of the congener, the
water content of the cells (freeze-dried versus frozen) and differences between field samples and
laboratory cultures. Variations in extraction efficiency may impact the accurate quantitation of
microcystins so the use of a surrogate compound to monitor the extraction efficiency is strongly
recommended. Responsible authorities should ensure that the appropriate methods and
preparation techniques  (extraction, concentration and separation) are being used in the laboratory
depending on the type of sample and the analytical method selected.

       Analytical methods available for the detection of microcystins in drinking water include
reversed phase high performance liquid chromatography (HPLC) coupled with mass
spectrometric (MS, MS/MS) or ultraviolet/photodiode array detectors (UV/PDA), Enzyme Linked
Immunosorbent Assays (ELISA), and Protein Phosphatase Inhibition Assays (PPIA).

       EPA has developed a liquid chromatography/tandem mass spectrometry (LC/MS/MS)
method for microcystins and nodularin (combined intracellular and extracellular) in drinking
water (Method 544; U.S.  EPA, 2015). Accuracy and precision data have been generated in
reagent water, and finished ground and surface waters for the following compounds: microcystin-
LA (microcystin-LA), -LF (microcystin-LF), -LR (microcystin-LR), -LY (microcystin-LY), -RR
(microcystin-RR), -YR (microcystin-YR), and nodularin-R (NOD). This method is intended for
use by analysts skilled in solid phase extractions, operation of LC/MS/MS instruments, and the
interpretation of associated data. The single laboratory lowest  concentration minimum reporting
levels (LCMRLs) for this method range from 2.9 to 22 ng/L (0.0029-0.022 |ig/L). The Detection
Limit (DL) for analytes in this method range from 1.2 to 4.6 ng/L. In this method, a 500 mL water


                Drinking Water Health Advisory for Microcystins-June 2015            38

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sample (fortified with an extraction surrogate) is filtered, and both the filtrate and the filter are
collected. The filter is placed in a solution of methanol containing 20% reagent water and held for
at least one hour at -20 °C to release the intracellular toxins from cyanobacteria cells captured on
the filter. The liquid is drawn off the filter and added back to the 500-mL aqueous filtrate. The
500-mL sample (plus the intracellular toxin solution) is passed through a SPE cartridge to extract
the method analytes and surrogate. Analytes are eluted from the solid phase with a small amount
of methanol containing 10% reagent water.  The extract is concentrated to dryness by evaporation
with nitrogen in a heated water bath, and then adjusted to a 1-mL volume with methanol
containing 10% reagent water. A 10-uL injection is made into an LC equipped with a C8 column
that is interfaced to an MS/MS. Analytes are separated and identified by comparing the acquired
mass spectra and retention times to reference spectra and retention times for calibration standards
acquired under identical LC/MS/MS conditions. The concentration of each analyte is determined
by external standard calibration. To download Method 544 Determination of Microcystins and
Nodularin in Drinking Water by Solid Phase Extraction and Liquid Chromatography/tandem
Mass Spectrometry (LC/MS/MS), please go to: http://www.epa.gov/nericwww/ordmeth.htm

       High performance liquid chromatography (HPLC) is widely used to separate microcystin
congeners. A variety of stationary phases have been used including reversed-phase Cig columns,
amide Cig columns, internal surface reversed-phase columns or ion exchange columns.
Optimization of chromatographic parameters is needed to ensure a good  resolution of analytes. In
addition to mass spectrometry, ultraviolet/visible absorbance is a commonly used detection
techniques with HPLC. Most microcystin congeners have similar absorption profiles between 200
and 300 nm. The wavelength of the UV/visible detector can be set at these values to record the
responses of microcystins in sample extracts separated by the HPLC. The retention time, UV
spectra and peak area of commercially available or laboratory standards is the basis of
identification and quantification of microcystins using HPLC-UV/visible detection. However, due
to the limited number of commercially available standards, the toxins are often quantified by
comparison to an microcystin-LR standard and reported in terms of microcystin-LR equivalence.
HPLC-UV/visible is susceptible to interferences from natural organic materials (NOMs).
Detection limits will depend partially on the sample volume extracted, the concentration of the
toxins, and the presence of interfering contaminants.

       A variety of antibodies have been isolated against microcystin-LR and microcystin-RR, as
well as recombinant antibody fragments and antibodies against the amino acid ADDA.
Commercial ELISA kits that contain all of the reagents needed for analysis have also been
developed and typically provide a cross reactivity chart for some of the congeners (i.e.,
microcystin-LR,  -RR, YR, nodularin) that are commonly found in water. These range from 50-
85% for microcystin-RR, 35-181% for microcystin-YR and  10-124% for microcystin-LA.
Detection of the total microcystins will be expressed as the sum of the congeners provided from
ADDA ELISA. The methods detection limit (MDLs) of several commercial laboratory ELISA
kits have been reported to range from 0.04 to 0.2 |ig/L for microcystin-LR. Commercial ELISA
kits generally have quantitation ranges from 0.2 (LOQ) to an upper limit of 5 |ig/L.  Two high
sensitivity ELISA plate kits have become commercially available with MDLs ranging from 0.04
to 0.05 |ig/L.
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       PPIAs are used with a variety of detection methods and substrates including radioactive
detection assays using 32P-radiolabelled substrates and colorimetric assays using p-nitrophenol
phosphate as the substrate. The method has also been adopted for fluorescence measurements
using the substrates methylumbelliferyl phosphate. The detection limit of total microcystins,
reported as microcystin-LR equivalents (microcystin-LRequiv) using radiometric protein
phosphatase assays is approximately 0.1 |ig/L or less, and using colorimetric PP1 inhibition
assays range between 10 to 20 ng/mL (0.01 to 0.02 |ig/L).

       Rapid tests for the identification of the presence of microcystins in water have been
developed for use in the field. Field test kits can be used as a presence/absence tool for
determining if a bloom is toxic or if treatment plant operations need to be adjusted during a bloom
event but do not currently have sufficient sensitivity at microcystin concentrations below 1 |ig/L
to be used for treated water analyses. Commercially-available test kits use a variety of methods
including immunochromatography (test strips), ELISA, and phosphatase inhibition to estimate the
level of microcystins in a water sample. In general, the results of field test kits should be
considered qualitative and should only be used to conduct a preliminary assessment of
microcystin levels. The applicability of test kits is between 1 and 5 |ig/L of microcystins with a
detection limit of approximately 0.5 |ig/L. Several field test kits do not include a lysing agent and,
therefore, only determine the presence of extracellular microcystins. When using these field test
kits, users should consult the manufacturer regarding an appropriate lysing technique if the
detection of both intracellular and extracellular microcystins is required.

       A new approach using laser diode thermal desorption-atmospheric pressure chemical
ionization interface coupled to tandem mass spectrometry (LDTD-APCI-MS/MS) has been
developed for the analysis of total microcystins in complex environmental matrices. The method
is based on oxidation of the MCs in a sample using potassium permanganate under alkaline
conditions to produce 2-methyl-3-methoxy-4-phenylbutyric acid (MMPB). MMPB is then
extracted and directly injected (no chromatographic separation) into the LDTD-APCI-MS/MS
system. This approach results in ultra-fast sample analysis with simple sample preparation,
reducing time and material costs associated with chromatographic separation. This method does
not require individual MC standards, but similar to ELISA and PPIA, the results do not provide
information on the identity of the individual MC congeners. The MDL and LOQ are 0.2 and 0.9
|ig/L, respectively (Roy-Lachapelle et al.,  2014).
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6.0 TREATMENT TECHNOLOGIES

       The information below is adapted from the Health Canada Guidelines for Cyanobacteria
Toxins in Drinking Water, available later in 2015.

       Detailed information on the operational considerations of a variety of treatment methods
can be found in the EP A Drinking Water Treatability Database for Microcystins (U.S. EPA,
2007); the International Guidance Manual for the Management of Toxic Cyanobacteria (GWRC,
2009) available at http://www.waterra.com.au/cyanobacteria-
manual/PDF/GWRCGuidanceManualLevell.pdf, and Management Strategies for Cyanobacteria
(Blue-Green Algae): A Guide for  Water Utilities (Newcombe et al., 2010) available at
http://www.researchgate.net/profile/Lionel_Ho/publication/242740698_Management_Strategies_for_Cyan
obacteria_(Blue-Green_Algae)_A_Guide_for_Water_Utilities/links/02e7e52d62273e8f70000000.pdf

       For additional information on treatment strategies commonly used or being considered by
water systems vulnerable to cyanotoxins, please see Recommendations for Public Water Systems
to Manage Cyanotoxins in Drinking Water (U.S. EPA, 2015b).
6.1     Management and Mitigation of Cyanobacterial Blooms in Source Water

       Algaecides can be applied to lakes and reservoirs to mitigate algal blooms, including
Cyanobacteria. In most cases, depending on the Cyanobacteria species present, the application of
algaecides has the potential to compromise  cell integrity releasing cyanotoxins into the source
waters. Chemical treatment to control blooms in drinking water sources in the early stages of the
bloom when cyanob acted al concentrations  are still relatively low (usually under 5,000 to 15,000
cells/mL) (WHO,  1999), are less likely to release significant cyanotoxin concentrations upon cell
lysis and is able to mitigate or prevent a cyanob acted al bloom from proliferating as the season
progresses. If harmful cyanobacterial blooms occur, utilities may take action to investigate
alternative source water sources, change intake locations or levels to withdraw source water with
minimal cyanotoxin concentrations, or investigate methods of destratification in the water source.
Purchasing water from a neighboring interconnected water system that is unaffected by the bloom
may also be an option for some systems.

       Clays and commercial products such as aluminum sulfate (alum) have been used for the
management of blooms in source waters.  Alum treatment efficiency depends on the alum dose
and the type of flocculant. Aeration and destratification have also been used to treat
cyanobacterial blooms, usually in smaller water bodies (from one acre to several tens of
acres). Active mixing devices, diffuse air bubblers, and other means of reducing stratification
have proven to be effective in controlling outbreaks and persistence of blooms in relatively small
shallow impoundments (around <20 feet deep). These strategies can be applied to the entire
source water body or to just a portion of the lake depending on the need, and size and depth of the
water body relative to the source water intake(s).

       Hydrogen peroxide (H2O2) has been used as an algaecide in source water because of a
rapid reaction time (90% of bloom collapsed in 3 days and 99% in 10 days), and environmentally
safe reaction products (oxygen and water) (Wang et al., 2012; Matthjis et al; 2012). The
                Drinking Water Health Advisory for Microcystins-June 2015            41

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drawbacks (aside from cell lysis) are that oxidant breakdown is so rapid that repeated applications
are needed. Further understanding of this technique is needed (Matthjis et al., 2012).

       The use of ultrasonic sound waves to disrupt cyanobacterial cells has also been
investigated as a potential source water treatment option (Rajasekhar et al., 2012). It is
environmentally friendly compared to chemical treatment strategies. The technique has also been
reported to be capable of degrading microcystin-LR (Song et al., 2005). Drawbacks include that
application frequencies are difficult to calculate and are system-specific; and that applications on
large scale require more powerful and, therefore, more expensive equipment. Sonication shows
potential for use in cyanobacterial bloom management, but further study to determine effective
operating procedures is needed before it can be considered as a feasible approach (Rajasekhar et
al., 2012).

       Excess nutrients  are thought to be a primary driver of cyanobacterial blooms. Long-term
prevention of cyanobacterial blooms likely requires reductions in nutrient pollution. Excess
nitrogen and phosphorus in aquatic systems can stimulate blooms and create conditions under
which harmful cyanobacteria thrive. Thus, managing nutrient pollution sources within a
watershed in  addition to waterbody-specific physical controls (in systems that are amenable to
those controls) tends to be the most effective strategy. Nutrient pollution can be from urban,
agricultural, and atmospheric sources and, therefore, reductions can be achieved through a variety
of source control technologies and best management practices.
6.2     Drinking Water Treatment

       Effective treatment of cyanotoxins in drinking water includes the evaluation and selection
of appropriate treatment methods. Any variation in treatment methods aimed at reducing toxins
concentrations need to be tailored to the type(s) of cyanobacteria present and the site-specific
water quality (e.g. pH, temperature, turbidity, presence of natural organic material (NOM), etc.),
the treatment processes already in place, and the utility's multiple treatment goals (e.g., turbidity
and total organic carbon (TOC) removal, disinfection requirements, control of disinfection by-
products (DBF) formation, etc.). Utilities need to have an understanding of the type and
concentration of cyanotoxins present in the source water and should conduct site-specific
evaluations such as jar testings and piloting in order to determine the most effective treatment
strategy. Potential target parameters include: chlorophyll-a, turbidity, cyanobacterial cells and
extracellular and intracelluar toxins.Care should be taken to avoid cell lysisTo remove both
intracellular and extracellular toxins from drinking water, a multi-barrier approach is required,
which may consist of conventional filtration for intracellular cylindrospermopsin removal and
additional processes such as activated carbon, biodegradation, advanced oxidation, and small-pore
membrane processes (e.g. nanofiltration and reverse osmosis), for the removal or oxidation of
extracellular cylindrospermopsin. The most effective way to deal with cyanobacteria cells and
their toxins, is to remove the cells intact, without damaging them, to prevent the release
of additional  extracellular toxins  into the water.
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6.2.1  Conventional Treatment for Microcystins

       In the absence of cell damage, conventional treatment employing coagulation,
flocculation, clarification (sedimentation or dissolved air flotation) and rapid granular filtration
can be effective at removing intact cells and the majority of intracellular toxins (cell bound)
(Chow et al.,  1998; Newcombe et al., 2015). However, if toxins are released into solution, a
combination of conventional treatment processes with oxidation, adsorption, and/or advanced
treatment needs to be considered to treat both intracellular and extracellular cyanotoxins.

       The efficiency of the conventional treatment processes to remove cyanob acted al cells and
intracellular microcystins has been shown to vary from 60 to 99.9%. Factors that impact removal
include the cyanob acted al species and cell density, coagulant type and dose, pH, NOM, and
operational parameters such as flocculation time, frequency of filter backwashing and clarifier
sludge removal (Vlaski et al., 1996; Hoeger et al., 2004; Jurczak et al., 2005; Zamyadi et al.,
2012a, 2013c; Newcombe et al., 2015).  Typically, 60 to 95% of cells and intracellular
microcystins can be removed during sedimentation with as much as 99.9% removal achieved
through filtration (Lepisto et al., 1994; Drikas et al., 2001; Hoeger et al., 2004; Newcombe et al.,
2015). The efficiency of coagulation and clarification for cell removal is dependent on pH,
coagulant type and dose and the morphological characteristics of the cyanobacteria. Rapid sand
filtration without pre-treatment (i.e., direct filtration, without coagulation/clarification) is not
effective for cyanob acted al  cell removal.

       If operated properly, conventional treatment (coagulation, flocculation, clarification and
filtration), does not cause cell lysis or increases in the extracellular microcystin concentrations of
treated water (Chow et al., 1998, 1999; Drikas, 2001; Sun et al., 2012). Drinking water treatment
plants utilizing conventional treatment followed by oxidation or activated carbon may remove
both intracellular and extracellular microcystins up to 99.99% of total microcystins to achieve
concentrations below 0.1  |ig/L in treated water (Karner et al., 2001; Lahti et al., 2001; Hoeger et
al., 2005; Jurczak et al., 2005; Rapala et al., 2006; Zamyadi et al., 2013a).  Conventional treatment
is generally considered to have limited effectiveness for the removal of the extracellular
microcystins. Therefore, additional processes such as adsorption, chemical oxidation,
biodegradation or reverse osmosis, and nanofiltration are required to remove extracellular
microcystins.

       Although microfiltration and ultrafiltration membranes can remove both cyanobacterial
cells and intracellular microcystins, removal of extracellular microcystins using ultrafiltration is
variable (35 to 70%) and microfiltration is not effective (Gijsbertsen-Abrahamse et al., 2006;
Dixon et al., 201 la, b). Nanofiltration and reverse osmosis membranes can achieve high removals
of intracellular and extracellular microcystins, from 82% to complete removal  (Westrick et al.,
2010; Dixon et al., 2010). Pore size, among others, is an important factor in removal efficiency
for these processes.

       Successful removal of cyanobacterial cells and intracellular  microcystins will depend on
proper operations of the conventional treatment processes (Hoeger et al., 2004; Dugan and
Williams, 2006; Ho et al., 2013; Zamyadi et al., 2012a, 2013c). Operational considerations for
removing cyanobacterial cells using coagulation, flocculation and clarification are similar to
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considerations for achieving effective particle removal. The appropriate coagulant and
coagulation pH should be determined through jar-testing to maximize cell removal. In jar-testing,
the NOM, chlorophyll-a, or cyanobactedal cell count can be used to optimize the coagulation
conditions for cyanobacterial cell removal (Sklenar et al., 2014; Newcombe et al., 2015).
Sufficient mixing should be provided at the point of chemical addition to ensure rapid and
uniform contact, and an appropriate mixing speed should be determined to optimize the
flocculation process (GWRC, 2009). It is important to minimize the potential for the
accumulation of cyanobacterial cells as scums at the surface of sedimentation basins and filters
(Zamyadi et al., 2012a, 2013c).

       Effective sludge removal from sedimentation/clarification processes is important to
minimize the release of intracellular and extracellular microcystins into the surrounding waters, as
significant cell numbers can accumulate within the sludge, and cells contained within the sludge
can lyse rapidly (Drikas et al., 2001; Ho et al., 2013; Zamyadi et al. 2012a). It has been reported
that accumulation of cyanobacterial cells and microcystins in clarifiers can lead to their
breakthrough into filter effluent. In addition, cell lysis can occur in the clarifier sludge, increasing
the extracellular concentration of microcystins in the treatment plant. Therefore sludge
management (decreased sludge age) in clarifiers  and increased frequency of backwashing of
filters is important because settled/filtered cells can remain viable and possibly multiply over a
period of at least 2 to 3 weeks. Within 1 day, some cells in the sludge can lyse and release NOM
and taste and odor compounds, in addition to cyanotoxins (Newcombe et al., 2015). Additionally,
backwash water from the filters may contain cyanobacterial cells and/or extracellular
microcystins; hence, care needs to be  taken if spent backwash water is recirculated to the
beginning of the treatment process to  prevent the reintroduction of cells and toxins into the
treatment train. Although longer filter run-times  are typically desirable between backwashing,
during periods of high algal concentrations, cells can accumulate in the filter, which can
potentially lead to a significant amount of extracellular microcystins released into the filtered
water.  The optimum balance between maximizing water production and minimizing the risk of
toxin breakthrough will be plant-specific.
6.2.2   Adsorption

       Adsorption processes, such as granular activated carbon (GAC) or powdered activated
carbon (PAC), are effective at removing extracellular microcystins but are not capable of
removing intact cells and intracellular toxins (Lambert et al., 1996; Newcombe, 2002; Newcombe
et al., 2003). Removal through adsorption depends on many factors including the type of activated
carbon used, the microcystin congener and water quality conditions. In general, mesoporous
carbons (such as chemically-activated wood-based carbons) are the most effective for the removal
of microcystins (Newcombe et al., 2010).  Other factors such as the type of microcystin  congener
present, the raw water quality (i.e., NOM and pH) and contact time affect microcystins  removal
efficiency when using activated carbon processes. In addition, shortened filter run times or filter
overload may happen during cyanobacteria blooms. Therefore, water treatment plants should
conduct jar-testing to determine the most effective activated carbon dose, type, and feed point
prior to the application without affecting other water quality parameters and treatment processes
(Skienaretal., 2014).
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       The performance of GAC filtration for extracellular microcystin removal depends upon
the empty bed contact time (EBCT), carbon age, carbon pore size, and raw water quality
characteristics such as NOM and pH, as well as the microcystin variant (Newcombe, 2002;
Newcombe et al., 2003; Ho and Newcombe, 2007; Wang et al., 2007). Solution chemistry can
also affect microcystin-LR adsorption onto GAC. Enhanced removal of microcystin-LR has been
observed at lower pH (2.5 versus 6.5) due to either precipitation or reduced solvency effect
(Pendleton et al., 2001).

       Removal of extracellular microcystins by PAC can be highly effective (up to 95%)
depending on the microcystin congener and concentration, the PAC  type and dose, the contact
time and the water  quality characteristics such as TOC (Newcombe et al., 2003; Cook and
Newcombe; 2008; Ho et al., 2011). According to Newcombe et al. (2010), a PAC dose of 20
mg/L and a contact time of at least 45 minutes should be considered for removal of most
extracellular microcystins (with the exception of microcystin-LA).
6.2.3  Chemical Oxidation

       Chemical oxidation using chlorine, potassium permanganate, or ozonation can be effective
at oxidizing extracellular microcystins, but can also impaired cell integrity, resulting in an
increase in concentrations of extracellular microcystins in drinking water. By applying
conventional filtration (or other filtration process) first to remove the majority of intact cells, the
extracellular microcystin concentration is less likely to increase due to cell lysis when water water
is treated with oxidants. In cases where pre-oxidation (oxidant applied anywhere along the
treatment process prior the filter influent) is practiced, it may need to be discontinued during an
algal bloom or adjustments to the oxidant type and doses may be needed to minimize cell rupture
prior to filtration (Newcombe et al., 2015).

       The effectiveness of chemical oxidation of microcystins depends on the type of oxidant,
dose, contact time, microcystin congener and water quality characteristics such as pH and
dissolved organic carbon (DOC) (GWRC, 2009; Sharma et al., 2012). Laboratory-scale
experiments have demonstrated that the general trend for the effectiveness of cyanobacterial cell
and extracellular microcystin oxidation to be: ozone>permanganate>chlorine>chlorine-based
oxidants  (Acero et al., 2005; Rodriguez et al., 2007a, b; Ding et al., 2010; Sharma et al., 2012;).
However, selection of the most appropriate oxidant for microcystins should be based on the
characteristics of each water source, the disinfection requirements, and potential formation of
disinfection by-products (DBFs) (Sharma et al., 2012).

       It is also important to recognize that the use of oxidants may result in the formation of
DBFs and should be considered when selecting a strategy for oxidizing microcystins (Merel et al.,
2010; Zamyadi et al., 2012b; Wert et al., 2013). For example, ozone and chlorine dioxide can
result in the formation of inorganic DBFs, such as bromate and chlorite/chlorate, respectively.
Additionally, modifying pre-oxidation practices may compromise other treatment objectives (e.g.,
turbidity  removal), and should be considered.
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        The oxidation of microcystins by chlorine has been found to be highly effective (>90%
removal) under experimental conditions (Ho et al., 2006a; Acero et al., 2008; Merel et al., 2009;
Sorlini and Collivignarelli, 2011). However, the effectiveness of chlorination on the oxidation of
microcystins depends upon the chlorine dose, contact time, pH, temperature, and other water
quality characteristics (Sharma et al., 2012). Several studies have found that microcystins are
efficiently oxidized if pH is maintained below 8, the chlorine dose is greater than 3 mg/L and  0.5
to 1.5 mg/L of free chlorine residual is present after 30 minutes of contact time (Nicholson et  al.,
1994; Acero et al., 2005; Ho et al., 2006a; Xagoraraki et al., 2006; Newcombe et al., 2010).
However, much higher chlorine doses (2 to 10 mg/L) are required to lyse the cyanobacterial cell
and then oxidize the previously cell-bound microcystins (Zamyadi et al., 2013b).

       The oxidation of microcystins in water by permanganate is one of the more effective
processes for oxidizing extracellular microcystins in water (Sharma et al., 2012). Rodriguez et al.
(2007a) exhibited a 90% oxidation of microcystin-LR at a dose of 1.0 mg/L, a contact time of 60
minutes, a pH of 8, and a temperature of 20°C. Complete oxidation occurred at a dose of 1.5
mg/L (Rodriguez et al., 2007a). Treatment plants considering potassium permanganate for
oxidation of microcystins should be aware that permanganate can discolor water when it is
present in excess of 0.05 mg/L. Therefore, dosage control and process monitoring (e.g., visual
inspection of the basin effluent color, measuring permanganate residual) is important in avoiding
consumer complaints (MWH, 2012).

       The oxidation of microcystins in water by ozone has been shown to be highly effective
(greater than 90% oxidation) in laboratory-scale studies (Rositano et al., 2001; Shawwa and
Smith, 2001; Brooke et al., 2006). The efficacy depends on temperature, pH, ozone dose, contact
time, and other water quality characteristics  such as DOC and alkalinity (Sharma et al., 2012).
Utilities should also be aware  that the use of ozone may result in the formation of bromate and
other DBFs.

       Monochloramine is a weaker oxidant than chlorine and is not an effective treatment
barrier for microcystins (Westrick et al., 2010).

       Most laboratory studies have found that chlorine dioxide (CICh) is not effective for
oxidizing extracellular microcystins (Kull et al., 2004, 2006; Ding et al., 2010;  Sorlini and
Collivignarelli, 2011) or cyanobacterial cells and intracellular microcystins (Ding et al., 2010;
Wert et al., 2014) at dosages (1-2 mg/L) and contact times typically applied to drinking water.
6.2.4       Other Filtration Technologies

       Biological filtration, using either biologically-active sand or activated carbon, has been
shown to be effective for the removal of extracellular microcystins in bench- and pilot-scale
studies (Keijola et al., 1998; Bourne et al., 2006; Ho et al., 2006b, 2008, 2012) and in limited full-
scale studies (Grutzmacher et al., 2002, Rapala et al., 2006). The removal of intact cyanobacterial
cells and their associated intracellular toxins through physical straining in slow sand filters has
also been documented (Grutzmacher et al., 2002; Pereira et al., 2012). Biological filters also have
the capability to remove particulate including intact cyanobacterial cells. Bank filtration may also
be effective for the removal of microcystins (Lahti et al., 1998; Schijven et al., 2002). A detailed


                Drinking Water Health Advisory for Microcystins-June 2015             46

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review of biological treatment options for cyanotoxin removal conducted by Ho et al., (2012b)
identified the type and concentration of microcystin-degrading bacteria, concentration of
microcystins, and temperature as key factors that influence the efficiency of biological filtration
for the removal of microcystins. In addition, the concentration of other organic matter within the
source water may inhibit biodegradation, as microcystins may be a secondary substrate in the
presence of NOM. Particle size, chemical composition and roughness or topography of the
surface of the media used for filtration have also been identified as important factors for biofilm
growth and ultimately the biodegradation of microcystins (Wang et al., 2007, Ho et al., 2012).

       Membrane filtration including microfiltration (MF) and ultrafiltration (UF) can achieve
greater than 98% removal of cyanobacterial cells and intracellular microcystins (Chow et al.,
1997; Gijsbertsen-Abrahamse et al., 2006; Campinas and Rosa, 2010: Sorlini et al., 2013).
Nanofiltration (NF), reverse osmosis (RO) and, to a lesser extent UF, can be used for both
intracellular and extracellular microcystin removal (Neumann and Weckesser,  1998; Lee and
Walker, 2008; Dixon et al.,  201 la,b). The performance of membrane filtration for microcystin
removal depends on characteristics of the membrane such as molecular weight cut-off (MWCO)
and hydrophobicity, initial concentration, size and molecular weight of the microcystins, and
operating parameters such as flux, recoveries and degree of fouling. It is recommended that
cyanobacterial cells are removed prior to reverse osmosis to prevent membrane clogging and
fouling.

       Laboratory and pilot-scale studies have demonstrated that MF and UF can remove greater
than 98% of cyanobacterial  cells (Chow et al., 1997, Gijsbertsen-Abrahamse et al., 2006;
Campinas and Rosa, 2010; Sorlini et al., 2013), and ultrafiltration can be moderately effective
(35-70%) for removal of extracellular microcystins (Lee and Walker, 2008). Several studies have
also demonstrated that the release of intracellular microcystins from the shear stress on
cyanobacterial cells during MF and UF is possible, although it generally results in permeate
microcystin concentration increases of less than 12 percent (Gijsbertsen-Abrahamse et al., 2006;
Campinas and Rosa, 2010).

       The removal of extracellular microcystins by NF and RO is very effective (greater than
90%) and depends on the MWCO, as the filtration of microcystins occurs  via size exclusion
(Gijsbertsen-Abrahamse et al.,  2006).
6.2.5       Combined Treatment Technologies

       In practice, full-scale treatment plants use a combination of treatment technologies (i.e.,
conventional filtration and chemical oxidation) in order to remove both intracellular and
extracellular microcystins. Data indicate that utilities can effectively remove both intracellular and
extracellular microcystins to achieve concentrations below 0.1 |ig/L (Lahti et al. 2001; Boyd and
Clevenger, 2002; Zurawell, 2002; Hoeger et al., 2005, Jurczak et al., 2005; Rapala et al., 2006;
Haddix et al., 2007; Nasri et al., 2007; Zamyadi et al., 2013c). However, some studies have
shown that the presence of high concentrations of cells (i.e., 105 cells/mL) and/or microcystins in
raw water (100 |ig/L) may be challenging for treatment plants to reduce concentrations to below
0.1 |ig/L (Tarczyriska et al., 2001; Zamyadi et al., 2012a).
                Drinking Water Health Advisory for Microcystins-June 2015            47

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       In most cases, utilities will be able to effectively remove intracellular microcystins with
processes that are already in place (e.g., conventional treatment) when they are operated with a
focus on cyanobacteria cell or NOM removal. Extracellular microcystins may also be removed in
many treatment plants by using existing treatment such as chlorination after filtration or by the
addition of PAC following conventional treatment (Carriere et al., 2010). Although it is possible
to remove both intracellular and extracellular microcystins effectively using a combination of
treatment processes, the removal efficiency can vary considerably. Utilities need to ensure that
they are utilizing their existing treatment processes to their fullest capacity for removal of both
cyanobacterial cells and extracellular microcystins and that appropriate monitoring is being
conducted to ensure that adequate removal is occurring at each step in the treatment process.
6.3  Point-of-Use (POU) Drinking Water Treatment Units

       Limited information is available on residential treatment units for the removal of
cyanobacteria cells and microcystins. A study using common water filtration and purification
systems found that the efficacy of POU filtration devices to remove microcystin (LR) varies
considerably with the type of device being used (Pawlowicz et al., 2006). Microcystin-LR was
successfully removed using carbon filters allowing only 0.05 to 0.3% of the toxin load to pass
through the filter. However, more than 90% of microcystin-LR passed through string-wound
filters and pleated paper. According to the authors, the use of carbon home filter devices tested in
this study may provide additional protection beyond that provided by the drinking water treatment
plant against human exposure to microcystin-LR. Additional studies are recommended to assess
the efficacy of POU drinking water treatment units for other cyanotoxins and under other
conditions. Third-party organizations are currently developing certification standards to test POU
devices to evaluate how well they remove cyanotoxins from drinking water treatment units. Those
standards are expected in the near future.

More information about treatment units and the contaminants they can remove can be found at
http://www.nsf.org/Certified/DWTU/.
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