Prepared
by
James N. Huckins
J.D. Petty
Jon A. Lebo
Carl E. Orazio
Randal C. Clark
Virginia L. Gibson
Limitations
of Conventional Sampling Sample Processing and Enrichment Residue
Residence (Retention) Time Appropriateness of Lipid Normalization back to Table of Contents |
SPMD |
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We gratefully acknowledge
the financial support of the Biological Resources Division of the U.S.
Geological Survey, U.S. Fish and Wildlife Service, the National Fish and
Wildlife Foundation, National Science Foundation, the American Petroleum
Institute, Chevron Oil Co., AMOCO Corp., and the Department of Defense.
We also appreciate the valuable contributions of Harry Prest, Robert
Gale, Kees Booij, John Meadows, Kathy Echols, Tom Johnson, Don Tillitt, and
Bruce Moring.
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of Contents
Researchers at the U.S.
Geological Survey's Columbia Environmental Research Center (CERC) developed and
patented (government) a technology that has diverse potential environmental and
industrial applications. The
technology is based on several different configurations of semipermeable
membrane devices (SPMDs). As
passive in situ devices, SPMDs can be used for contaminant monitoring,
exposure and toxicity assessment, and can also be used for analytical
separations. Although SPMD
technology is becoming widely accepted, the literature provides little guidance
on using SPMDs. This document
emphasizes the in situ concentration of contaminants for exposure and
toxicity assessments and provides a brief tutorial for scientists.
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Semipermeable Membrane Devices (SPMDs)
Lipid-containing SPMDs
represent an innovative passive sampling technology for monitoring and assessing
trace levels of hydrophobic organic contaminants.
The SPMD is typically constructed from barefoot (no additives) layflat
tubing of low-density polyethylene (LDPE).
The thin-walled (<100 µm) LDPE tubing used in SPMDs is normally
described as nonporous. However,
random thermal motions of the polymer chains form transient cavities with
maximum diameters of approximately 10 Å. Because
these cavities are extremely small and dynamic, hydrophobic solutes are
essentially solubilized by the polymer. The cross-sectional diameters of nearly all environmental
contaminants are only slightly smaller than the polymeric cavities.
Therefore, only dissolved (i.e., readily bioavailable) organic
contaminants diffuse through the membrane and are concentrated through time.
The sequestration media consist of both the thin film/plug of a large
molecular weight (> 600 daltons) neutral lipid such as triolein and the LDPE
membrane. Contaminant residues
concentrated in SPMDs are simultaneously recovered and separated from the lipid
in intact SPMDs (after carefully cleaning exterior surface of the membrane) by
dialysis in an organic solvent.
SPMDs accomplish three
tasks simultaneously:
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Mimics the
bioconcentration of organic contaminants in fatty tissues of organisms |
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Provides a
highly reproducible passive in situ sampler for monitoring
contaminant levels, which is largely unaffected by many environmental
stressors that affect biomonitoring organisms |
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·
Enables in
situ concentration of trace organic contaminant mixtures for toxicity
assessments and toxicity identification evaluation (TIE) |
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Limitations
of Conventional Sampling Methods
1.
Analysis of
excised water and air samples reflects residue composition only at the moment of
sampling and may fail to detect episodic contamination
2.
Quality control
and physical difficulties are often encountered when large volumes of water and
air must be collected and extracted for quantifying and assessing trace organic
contaminants
3.
Concentrations
of truly dissolved or readily bioavailable contaminants are not accurately
measured by most conventional approaches
4.
Aquatic
toxicity data, and threshold limit values for airborne exposures are based on
dissolved or vapor phase concentrations, not total residue levels
5. Standard low volume (< 4 L) techniques often fail to detect trace levels of bioconcentratable contaminants and seldom recover enough residue mass for bioassays
6.
Biomonitoring
organisms may not accurately reflect environmental contaminant concentrations,
because of residue metabolism/depuration and the effects of environmental
stressors on organism health
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SPMD Approach to Contaminant Monitoring
Although passive
diffusional monitors are widely accepted as the best method for determining
occupational exposure of workers to ambient organic vapors, this type of
integrative, or time-weighted average (TWA) approach has seldom been applied to
concentrating / measuring trace contaminants in aquatic environments. Passive integrative samplers act as infinite sinks for
accumulated residues, i.e., no significant losses of sequestered residues occur
even when ambient chemical concentrations fall during part of an exposure.
The following characteristics apply to SPMDs:
1.
The SPMD uptake
of contaminants with log KOWs > 4.9 is usually integrative or
linear (equilibrium not approached) during exposures £
30 days, and SPMD concentrations are proportional to ambient environmental
concentrations
2.
For organic
compounds with log KOWS < 4.9, equilibrium concentrations of
analytes may be reached or approached in < 30 days, but SPMD levels
are still proportional to those in the sampled medium
3.
Integrative
sampling reduces the probability of false-negatives, i.e., residues sequestered
from episodic events are retained and thus can be detected
4.
Laboratory
calibration (standard SPMD configuration) is required for estimating TWA ambient
chemical concentrations from SPMD levels and these data are already available
for several chemical classes
5.
Only dissolved
or vapor phase (readily bioavailable) organic pollutants diffuse through or are
sampled by the polymeric films or tubes used in SPMDs (e.g., LDPE and Silastic®)
6.
SPMDs mimic key
mechanisms in contaminant bioconcentration; these include (a) the passive
processes of contaminant diffusion through biomembranes (primarily the gill
epithelium in fish) and (b) partitioning between an organism's lipids and the
surrounding medium
7.
The triolein
used in SPMDs is a neutral lipid found in most aquatic organisms
8.
Because SPMDs
are constructed of synthetic materials, they are more uniform and sample more
reproducibly than biomonitoring organisms
9.
Although a
combination of laboratory calibration data and the use of
permeability/performance reference compounds (PRCs, see subsequent description
of these QC standards) in deployed SPMDs are usually required for accurate
estimates of contaminant concentrations in ambient media, the necessary
information is available in several recent publications cited herein
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General Specifications of SPMDs
Membranes:
Thin-walled (50-100 µm)
nonporous polymer film or tubes consisting of
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·
LDPE (low
density polyethylene) |
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·
Silicone
or Silastic (option of plasma-treated surface) |
|
·
Polypropylene |
|
·
Ethylene vinyl
acetate |
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·
Others |
Potential sequestration phases:
Large molecular weight (»
600 daltons) nonpolar liquids or fluids such as
|
·
Neutral
lipids |
|
·
Silicone
fluids |
|
·
Other
lipid-like organic fluids |
|
·
The LDPE
membrane alone |
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Standard SPMD Configuration (Commercially Available)
Membrane:
LDPE layflat tubing
manufactured without additives
Sequestration phases:
High-purity synthetic
triolein (>
95%)
and the LDPE membrane
Dimensions (specifications):
Generally 2.5-cm wide (layflat)
by 91.4-cm-long LDPE tubes (70-95 µm wall thickness and surface area is »
450 cm² or » 100 cm²/g
SPMD) containing 1 mL (0.915 g) of triolein as a thin film.
Other lengths and widths can be used if the lipid-to-membrane mass ratio
is maintained at » 0.2 and the membrane thickness is within the above
range.
Note:
Nearly all SPMD calibration data are based on the standard SPMD.
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Commercial Availability
SPMD technology is the
subject of two government patents (Huckins et al., U.S. Patents, #5,098,573 and
#5,395,426) that were licensed to Environmental Sampling Technologies (EST), a
division of Custom Industrial Analysis Labs, 1717 Commercial Drive, St. Joseph,
MO 64503. The patents cover both
assembly of SPMD and dialytic recovery of analytes from SPMDs.
Various SPMD configurations and deployment apparatuses are available from
the manufacturer. The European
source of SPMDs is ORIGO Hb, Trehorningen 34, S-922 66 Travelsjo, Sweden.
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SPMD Assembly and Quality Control Considerations
Assembling SPMDs requires
considerable care to ensure that the finished product is free of contaminants.
For sampling trace contaminants, the following quality control procedures are
adhered to during SPMD manufacture:
1.
Synthetic
triolein or lipid is used. All new
lots or batches are analyzed for contaminants, ampulated, and stored in a
freezer until use
2.
A micropipettor
is equipped with a total displacement plunger to accurately deliver small
volumes of triolein
3.
Just before use
in SPMD construction, SPMD tubing is batch-extracted with nanograde hexane or
cyclohexane
4.
To enclose
triolein in SPMD layflat tubing, a heat sealer (e.g., the "Seal a Meal®"
bag sealer) is used to create a molecular weld
5.
Because SPMDs
are extremely efficient air samplers (PCB sampling rates for a 1-g triolein SPMD
often approach and can exceed 10 m3/day), all assembly operations are
conducted in an environmentally controlled chamber (clean room) with both vapor
and particulate phase filters
6.
After assembly,
SPMDs are sealed in gas-tight clean paint cans (solvent rinsed to remove cutting
oils) for transport to deployment site
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|
·
Non-mechanical,
passive device which is easy to deploy and requires no maintenance |
|
·
Mimics
uptake of dissolved contaminants by biota, yet precision of concentration
data is greater |
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·
SPMD
matrices can conveniently be cleaned up prior to use, while extensive
depuration periods may be required to reduce contaminant levels in the
tissues of biomonitoring organisms |
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·
Readily
concentrates contaminant residues such as PAHs that are metabolized by
many aquatic organisms |
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·
Once
prepared, SPMDs can be stored frozen until the most appropriate deployment
time, while biomonitoring organisms require care and feeding, and may be
subject to seasonal availability |
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·
Analytical
cleanup of exposed SPMDs is generally less difficult than biomonitoring
organism tissues or sediment samples |
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Applications
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·
Determination
of pollutant sources and relative levels |
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·
Detection
of episodic chemical releases |
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·
Measurement
of TWA concentrations of dissolved or vapor phase chemical concentrations |
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·
Determination
of the readily bioavailable fraction (dissolved or vapor phase) of a
chemical in an environmental compartment for predicting transport, fate,
and residue toxicity |
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·
Estimation
of organism exposure and bioconcentration |
|
·
In
situ
biomimetic extraction of environmental contaminants for bioassay and
immunoassay |
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·
Dialytic
separations (SPMD membrane) of target analyte interferences in various
matrices |
|
·
Tool for
TIE procedures |
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Specifics of SPMD Sampling
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· Using the standard SPMD configuration with the LDPE membrane, only nonionic compounds are extracted or sampled because of the lack of membrane permeability by charged species |
|
· In general, molecules of organic compounds must be dissolved or in the vapor phase to be sampled by the LDPE SPMD membrane |
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· SPMD linear uptake rates are expressed as the daily volume of water or air cleared of chemical by an SPMD, given in units of L or mLd-1, L or mLd-1g-1 and m³ d-1 g-1, respectively, and are independent of concentration |
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· Theory and experimental data suggest that under relatively quiescent conditions (< 1 cm/sec, flow velocity at membrane surface) and moderate temperatures (i.e., 18-26ºC), the aqueous sampling rate of a 4.5 g standard SPMD (defined earlier) for most hydrophobic compounds ranges from about 0.5 to 10 L/d |
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· Sampling rates can be affected by the physicochemical properties of the target compound (i.e., octanol-water or -air partition coefficient [KOW or KOA], polarity, molecular size/weight, and volatility) and environmental conditions of the exposure site (i.e., temperature, flow/turbulence, and biofouling level or the growth of a biofilm on the exterior membrane surface) |
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· The driving force for uptake is directly related to the magnitude of a chemical's KOW/KOA or more specifically the KSPMD (equilibrium SPMD-water or -air partition coefficient) and for hydrophobic compounds the overall resistance to chemical uptake or mass transfer is inversely proportional to medium flow/turbulence, and directly proportional to the thickness of the aqueous boundary layer and the membrane (only when uptake controlled by membrane) |
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· For exposure conditions of low to moderate flow/turbulence, SPMD uptake is under membrane control for compounds with log KOWs < 4.4 and under aqueous boundary layer control for compounds with log KOWs > 4.4 |
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· Sampling rates are unaffected by aqueous flow/turbulence only when a chemical is completely under membrane control |
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· Temperature affects sampling rate, regardless of which step in the uptake process is rate limiting or has the most resistance to mass transfer |
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· Given the wide range environmental exposure conditions, flow/turbulence effects are generally expected to have a greater impact on SPMD sampling rate than temperature or biofouling |
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· The capacity or the total volume of water or air extracted by an SPMD at equilibrium is given by KSPMD MSPMD (where KSPMD is expressed as L, mL or cm³/g and MSPMD is the mass of the whole SPMD in g) and is roughly equivalent to KOW or KOA times MSPMD |
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· The KOW or KOA can be viewed as the approximate volume (mL, cm³, or L) of water or air extracted by one g of SPMD at equilibrium |
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·
Depending
on a compound’s KOW, residue uptake is representative of one
of three phases (see subsequent figure): linear or integrative (i.e., no
significant losses of accumulated residues, equilibrium not approached
during the exposure), curvilinear (partly integrative, equilibrium
approached) and equilibrium (the amount of chemical taken up is exactly
equal to the amount of chemical lost, per unit time) |
|
· Ambient exposure conditions affect sampling as described in the "SPMD sampling" subsection |
|
· Exposure duration is a major factor in the total amount of chemical accumulated |
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· Water or air concentration of target compound also affects the amount of chemical accumulated but not its uptake rate (i.e., the daily volume of an medium cleared of chemical) |
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Examples of Contaminants That are Significantly
Concentrated in Triolein-Containing SPMDs (not all-inclusive)
1.
Polychlorinated
dioxins and furans
2.
Polycyclic
aromatic hydrocarbons (PAHs)
3.
Polychlorinated
biphenyls (PCBs)
4.
Organochlorine
insecticides
5.
Pyrethroid
insecticides
6.
Several
herbicides and many industrial chemicals
7.
Alkylated
selenides
8.
Tributyl tin
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Mass of an Analyte Sequestered by an SPMD Depends on
1.
SPMD sampling
rate; higher temperatures (water) and flow rates/turbulence generally
provide higher SPMD sampling rates
2.
Water or air
concentration during interval of exposure
3.
Exposure
duration
4.
Level of
fouling or coating of the exterior membrane surface
Note:
Assuming background concentrations are very low in SPMDs, the investigator can
increase the number of SPMDs or exposure length (caveat: during long
exposures fouling often diminishes uptake rates) to increase the mass of
sequestered analytes.
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Size and Number of SPMDs Needed for a Project Depend
on
1.
Detection and
quantitation limits desired by the investigator
2.
In situ
SPMD sampling rate for the chosen analytes
3.
Average water
concentration of the analytes during the exposure interval
4.
Sensitivity and
selectivity of the chosen analytical method or bioassay
5.
Single or
multiple points in time (time resolution desired)
6.
Replication or
statistical requirements; the coefficient of variation (C.V.) of contiguous
replicate SPMDs is typically < 20%
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General Comments on Deployment Methods
|
·
Typically,
SPMDs are stored and shipped in clean gas-tight metal cans of various
sizes |
|
·
Metal
containment structures (storage cans and deployment devices) must be free
of cutting oils or other potential interferences |
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·
Minimize
use of plastic components, except Teflon and some types of PVC, due
to the possible presence of leachable organic residues |
|
·
The
structural design of the deployment device should minimize abrasion of the
membrane even in turbulent environments while baffling the very high
flow/turbulence of some media |
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·
Current
velocity/turbulence is also a concern in terms of tethering, especially
during floods |
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·
If a loop
design (SPMD) is used, the two sides should not make contact |
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·
If water
turbidity is low, then a shading structure may be required for analytes
such as PAHs that undergo photolysis (caution: estimated photolysis
half-lives of PAHs in direct sunlight range from 0.1 h to 5 h) |
|
·
For
sampling PAHs from air, the deployment structure must reduce ambient
sunlight levels to near zero |
|
·
Unless
permeability/performance reference compounds (PRCs) are used (see
description of PRCs in subsequent section), the flow and temperature
regime of exposure sites should be similar to facilitate inter-site
comparisons |
|
·
Because
vandalism is always a potential problem in the field, the deployment
structure should be amenable to hiding |
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·
Deployment
structures are commercially available (see "example of deployment
structure") |
A
commercially available stainless steel deployment apparatus, which has a
capacity for 5 standard SPMDs. Each
SPMD is placed on a separate rack and the five racks are held in place by a
threaded center pin as shown in the picture.
Also pictured are gas tight steel cans used for transport and storage.
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Recovery and Storage of SPMDs
1.
As soon as
SPMDs are recovered from the environment, they should be sealed in the original
can and placed on ice in a cooler for shipping (overnight shipping is
recommended)
2.
Some loss of
SPMD-sequestered analytes with high Henry's constants (> 10-3
atm-m3/mole) and low KOW values (£
1 x 103) is possible but should be minimal when compared to excised
water samples
3.
SPMDs should be
stored in the sealed cans (shipping containers) in a freezer at -20 o C
until analysis
4.
To ensure the
validity of this storage method, a relatively high fugacity (escaping tendency)
compound (2,4,5-trichlorophenol) was spiked into several SPMDs and the devices
were left open in a freezer; no losses were measurable after 6 months
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Preparation for Analysis
1.
To permit
dialytic recovery of residues in the SPMD membrane and lipid, the periphyton,
mineral precipitates, and sediments/soot (air) must be removed from the exterior
membrane surface (see Huckins
et al., [1996] for cleaning procedure)
2.
Membrane
cleaning is not necessary if only the lipid is analyzed or assayed
3.
After cleaning,
check for holes in the membrane to ensure the sampler’s integrity
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Comments on Analyte Enrichment Required
For
Analysis or Assay of Residues in SPMDs
1.
Analyte
recovery and enrichment procedures for SPMDs generally require less effort than
those for tissue and sediment matrices
2.
Similar to all
other environmental matrices, recovered analytes that are members of complex
mixtures typically require class fractionation (not necessary for bioassay)
after cleanup of any SPMD-related lipids, polyethylene waxes, and other
interferences
3.
SPMD extracts
are readily amenable to a classic TIE approach to elucidate the identity of
toxicants
Petty et al. (2000)
have discussed analytical methods required for SPMD analysis. The following
figures illustrate general procedures used for the recovery/cleanup of target
analytes or unknowns from SPMDs.
For more details on
sample processing and enrichment, see References.
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Sampling Rate Determination
Selected SPMD Aqueous Sampling
Rates (RS, Standard 1-g Triolein SPMD) for Nonpolar Organic
Contaminants1
Chemicals |
Rs L/d |
Log Kow |
Acenaphthylene |
1.4 |
4.2 |
Flourene |
1.7 |
4.4 |
Pyrene |
5.2 |
5.3 |
Chrysene |
4.8 |
5.6 |
Benzo[a]pyrene |
3.7 |
6.4 |
Lindane |
0.72 |
3.9 |
p,p’-DDT |
3.6 |
6.2 |
Endrin |
3.2 |
5.5 |
Trans-nonachlor |
1.9 |
5.6 |
Hexachlorobenzene |
2.7 |
6.4 |
2, 2’,5, 5’-Tetrachlorobiphenyl |
4.9 |
5.6 |
1
Flow-through (< 1 cm/sec velocity) constant concentration (100 ng/L)
exposures at 18 °C; biofouling was minimized
2 Value based on 4-d exposure; uptake not linear/integrative after 6
days
Note: for a much
more extensive listing of sampling rates see Huckins et al., Guide for
the use of SPMDs as samplers of waterborne hydrophobic organic contaminants, API
no. 4690, In press.
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Requirements for Estimating Ambient Contaminant
Concentrations from SPMD Concentrations
1.
Laboratory
determination of SPMD exchange rates (uptake and elimination) and KSPMDs
for analytes of interest at multiple temperatures
2.
Analyte
concentrations in whole SPMDs through time is recommended when feasible
3.
Average
temperature during the exposure
4.
Flow velocity
5.
Estimates of
possible reduction in sampling rate due to fouling
Note:
Use of PRCs should negate the need for requirements 4 and 5.
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Huckins et al. (1993)
described the basic theory related to the uptake and dissipation of contaminants
from SPMDs and development several mathematical models for estimating water
concentrations from analyte concentrations in SPMDs.
SPMD sampling rates were demonstrated to be independent of water
concentration, while the amount of accumulated residues is proportional to the
concentrations of dissolved chemicals.
Modeling
Assumptions and Overall Exponential Model
Using a lipid-equivalent
approach to model the contribution of the membrane, and making no initial
assumptions about the rate-limiting step in the overall SPMD uptake process,
analyte concentrations in water and air can be computed from the following
relationship.
CW,
A = CSPMD / KSPMD (1-exp [-ket])
Equation 1
Where CW, A is
the analyte concentration in water or air, CSPMD is the analyte
concentration in the SPMD, t is time, KSPMD is the equilibrium
SPMD-water or -air partition coefficient, and ke is the first-order
loss rate constant. This model fits
the overall uptake curve (see figure illustrating the three phases of SPMD
uptake), but is primarily used for compounds that reach the curvilinear uptake
phase during an exposure. Based on equation 1, it appears the rate that
chemicals are accumulated by an SPMD is dependent on the loss rate (ke)
of residues from the device, which has units of t-1.
Actually, ke is dependent on both the uptake rate constant and
the KSPMD as shown by
ke =
ku / KSPMD
Equation 2
where ku is the
linear uptake rate constant given in L/d·g, and this case, KSPMD has
units of L/g. Isotropic exchange
kinetics (IEK) are implicit in both equations 1 and 2, which means that the
overall process of residue uptake and elimination obeys the same rate law, and
that measured in situ PRC kes values (along with KSPMD
values) can be used to predict in situ kes, and thus kus
of the analytes of interest. However,
use of equation 1 without curve fitting software (requires multiple points in
time) is dependent on knowledge of CSPMD, KSPMD, and ke
or ku.
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Estimation
of KSPMD
Because the SPMD
consists of two phases (i.e., lipid and membrane) that accumulate residues, the
KSPMD is given by
KSPMD
= (KMW VM + KLW VL) / VSPMD
= KLW (VL + KML VM) / VSPMD
Equation 3
Where
Kmw is the equilibrium membrane-water partition coefficient, Vm
is the volume of the membrane, KML is the equilibrium membrane-lipid
partition coefficient, VL is the volume of the SPMD lipid, and VSPMD
is the total volume of the SPMD. Unfortunately,
only a few values of KSPMD are available for air.
By assuming that KSPMD remains constant within the typical
range of environmental exposure temperatures, Equation 3 and two regression
models developed by Hofmans (1998) can be used to compute KSPMD.
These regression models are as follows:
log
KLW = -0.1257 (log KOW)² + 1.9405 (log KOW)-1.46
Equation 4
and
log
KMW = -0.0956 (log KOW)² + 1.7643 (log KOW)
–1.9
Equation 5
Note
that the accuracy of the equations above diminishes at log Kows >
6.0 and that SPMD aqueous partition coefficients can be converted into SPMD air
partition coefficients by dividing each value by the corresponding
non-dimensional Henrys constant (H'), which are generally available in the
literature.
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Linear
Uptake Model (Integrative Sampling Phase)
For
high KOW compounds (i.e., log KOW > 5.0), uptake
is generally linear during non-turbulent, moderate temperature exposures (note
that biofouling impedance in some aquatic environments may cause a deviation
from linearity during longer exposures). When
uptake is linear, CW, A can be derived from CSPMD by the
following relationship
CW,
A = CSPMD MSPMD / Rs t = CSPMD
/ ku
Equation 6
where
MSPMD is the mass of the SPMD in g and Rs (L/d) is
operationally defined as the sampling rate of a "standard" 1-g
triolein SPMD. The advantage of
this type of sampling (integrative) is that residues are accumulated through
time without any significant losses (permits the maximum sequestration of target
compound mass), and estimates of analyte levels from Equation 6 represent true
TWA concentrations.
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Equilibrium
Model
For
compounds with moderate to low KOW s (i.e., log KOW <
5.0), and when exposure conditions are relatively turbulent and warm, residue
concentrations may closely approach (i.e., ³
90 %) or reach equilibrium concentrations in SPMDs.
In this case, the following model is applicable to the estimation of
ambient environmental concentrations.
CW,A
= CSPMD-e /KSPMD
Equation 7
where
CSPMD-e is the equilibrium concentration of an analyte in the SPMD.
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Estimation
of Times for the Phases of SPMD Uptake
In
the absence of PRC data, selection of the appropriate model for estimation of
ambient concentrations from SPMD concentrations is problematic.
However, the following equations can be used to provide some guidance.
t50
= t1/2 = -ln 0.5 KSPMD VSPMD / Rs =
-ln 0.5 KSPMD / dSPMD ku
Equation 8
t90
= -ln 0.1 KSPMD VSPMD / Rs = -ln 0.1 KSPMD
/ dSPMD ku
Equation 9
t1/2
»
-ln 0.5 KOW VSPMD
/ Rs »
-ln 0.5 KOW / do ku
Equation 10
where
t50 is the time required to accumulate 50 % of the equilibrium
concentration, and is mathematically identical to t1/2 (time required
to lose 50 % of the initial residue concentration), t90 is the time
required to reach 90 % of the equilibrium concentration, and dSPMD
and do are the density of the whole SPMD (» 0.91 g/cm3) and octanol. Note that the first 50 % of the total residue accumulated
essentially represents the linear region of uptake, > 50 % to 90 % represents
the curvilinear region, and > 90 % represents the steady state or equilibrium
region. If the KSPMD and
KOW are written as unitless coefficients, the density corrections are
unnecessary. KOWs are
widely available and a considerable number of SPMD Rs and/or ku
values are now available in the "Guide For The Use Of Semipermeable
Membrane Devices (SPMDs) As Samplers Of Waterborne Hydrophobic Organic
Contaminants" by Huckins et al. (2001). See the following subsection on PRCs for a discussion on how
the amount of PRC loss during an exposure can be a guide for the choice of the
appropriate model for water or air concentration estimates.
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Permeability/Performance
Reference Compounds
As
previously indicated, PRCs are (analytically) non-interfering compounds with
moderate to relatively high fugacity from SPMDs, which are added to the SPMD
lipid prior to deployment. We use
"permeability" to refer to compounds under membrane control and
"performance" to refer to compounds under external boundary layer
control. The use of PRCs can be
viewed as an in situ calibration/recalibration approach, where the rate
of PRC loss during an exposure is related to the target compound uptake.
This is accomplished by measuring PRC loss rates (kes) during
calibration studies and field exposures. Using
these values, an exposure adjustment factor (EAF) can be derived.
The EAF, along with kus and kes from calibration
studies can then be used to predict in situ SPMD kus of
environmental contaminants. A
fundamental assumption of the PRC approach is that the EAFs of PRCs with log KOWs
generally < 5.0, can be used to predict the EAFs of chemicals with
much higher log Kows. Based
on a recent study by Huckins et al. (2002), this assumption appears valid and
the difference between measured concentrations of an analyte and the PRC derived
estimates should be within two fold.
When
temporal losses of PRCs are measured (n > 3), regression analysis can
be used to determine PRC ke values.
CSPMD
= CSPMD-0 exp (-ke-PRC t)
Equation
11
where
CSPMD-0 is the initial
PRC concentration. Generally, a
field blank containing a PRC is used to determine CSPMD-0.
If PRC levels in SPMDs are measured only at the beginning and the end of
a field exposure, Equation 11 can be solved to permit a two-point
derivation of ke-PRC s (assuming first-order kinetics) as follows:
ke-PRC
= ln (CSPMD-0 / CSPMD) / t
Equation 12
and
the EAF is derived by
EAF
º
ke-PRC-f / ke-PRC-cal »
(ku-f / KSPMD -f) / (ku-cal / KSPMD-cal)
Equation 13
where
“-cal” and “-f” refer to values measured during calibration studies and
in the field. The ku-f
(i.e., an estimate of the actual in situ sampling rate of the target
compound during a field exposure) can be derived by
ku-f
» KSPMD-f EAF (ku-cal
/ KSPMD -cal)
Equation 14
Selection
of compounds to serve as PRCs is limited by the need to have measurable losses
of PRC residues during an exposure and the ability to differentiate PRC residues
from other quality control standards, target compounds and unknowns of potential
interest to an investigator. Depending
on the Kows of target analytes, candidate PRCs may have to include
compounds that are representative of both membrane and diffusion control.
Also, some information on general environmental conditions (e.g., flow
rate and temperature) at sample sites and the duration of planned exposures are
advisable to help ensure that an acceptable range of PRC loss occurs during
exposures. For example, PRC losses
are enhanced under exposure conditions of warm turbulent waters.
To prevent the complete loss of PRCs under this scenario, the use of
compounds with moderately high log Kows (i.e., range of 4.5 to 5.3)
may be necessary and/or exposure length may have to be shortened.
In addition, larger quantities of these PRCs and those with low log KOWs
(i.e., < 3.5) may have to be spiked into SPMDs.
These precautions are necessary to ensure that changes in PRC residue
concentrations can be statistically delineated from the C.V.s (%) for SPMD
sample analyses. Even when PRC loss
or retention is too great to use for the derivation of EAFs, information on the
kinetic phase of analyte uptake (see figure on the three phases of SPMD uptake)
at the termination of the exposure is still gained (Booij, 2000).
For example, if a PRC with a log Kow of < 4.5 is completely
lost during an exposure, then all analytes with log KOWs of < 4.5
should have attained equilibrium (i.e., KSPMD-e).
On the other hand, if no loss of a PRC with a log Kow of >
5.0 is observed then linear uptake can be assumed for all analytes with log Kow
of > 5.0.
The
use of certain perdeuterated (all hydrogen atoms replaced with deuterium atoms)
compounds appears to offer considerable promise as PRCs.
This type of labeled compound is commercially available at relatively low
cost (when compared to similar 13C-labled compounds), has
physicochemical properties (excluding molecular weight) similar to their native
analogues, is not found at significant levels in the aquatic environment, and
generally can be separated from their native analogues by high-resolution gas
chromatography. Based on our
experience, the following perdeuterated PRCs are recommended: naphthalene,
acenaphthene and fluorene for membrane controlled analytes and phenanthrene,
anthracene and pyrene for diffusion layer controlled analytes. Note that if PAHs are used for PRCs or are target analytes,
exposure of SPMDs to sunlight must be avoided because they readily photodegrade.
When analyses are performed by mass spectrometry, then it is feasible to
use 13C -PRCs if appropriate standards
can be found at a cost within budget of the project.
Obviously, non-labeled compounds, such as 2, 2'-dichlorobiphenyl and 2,
4, 5-trichlorobiphenyl (not present in commercial PCB mixtures), can be used for
PRCs as long as they are not present in the environment sampled and are not used
as analytical quality control standards.
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SPMD-Biota Comparisons
These two plots show
the similarity of the uptake of a wide range of contaminants by SPMDs and the
gills of fish. In both cases,
uptake rates peak between log KOWs of 5.0 and 6.5 and the overall
shape of the curve appears to be parabolic.
This plot shows that
for high KOW compounds such as PCBs, uptake is similar and linear
(integrative) for both SPMDs and fish. However, standard-SPMD uptake rates of
total PCB congeners were about 1.8 fold higher than uptake rates of the test
fish and the capacity (i.e., equilibrium mass of analyte accumulated divided by
mass of the sampling matrix) of SPMDs is greater than fish.
Numerous
chromatograms of SPMD extracts, such as those above, show proportionally greater
quantities of nonpolar low molecular weight or low KOW chemicals
sequestered in SPMDs than in biota.
Because
of the seeming bias (relative to most biomonitoring organisms) of SPMDs to
accumulate larger amounts of low KOW compounds (log KOW
< 4.5) relative to high KOW compounds (log KOWs >
6.0), the following question arises: are SPMD sampling rates for
hydrophobic chemicals of low molecular weight greater than those for hydrophobic
chemicals of moderate-to-high molecular weight?
Before answering
this question, we should review the meaning of “sampling rate”. SPMD
sampling rates, Rs and ku, are given in Ld-1 (Rs)
or Ld-1g-1, which are first-order rate constants
independent of water concentration. These
rate constants represent a characteristic volume of water that is daily cleared
of chemical by an SPMD (lipid plus membrane).
SPMD Rs and ku
values have been shown to rise with KOW or molecular size until
boundary layer control is evoked (log KOW »
4.5). Then, falling diffusion rates with increased MW and potential solubility
and sorption limitations, significantly reduce RSs or kus
(appears to be evident at log KOW »
6.0). In general, sampling rates
for low KOW compounds are still less than those for moderate to high
KOW compounds. However,
this observation does not
mean that greater amounts of low KOW chemicals will not be
sequestered when water concentrations are much higher.
For example, environmental water concentrations of low KOW
compounds may often be 1000-fold greater than high KOW compounds,
whereas the SPMD ku values for the same compounds differ by only
about 30-fold. The amount of
analyte recovered in an SPMD (Ma) is given by
Ma
= ku MSPMD t Cw
Equation 15
Where Ma is the
mass of analyte sequestered. Therefore,
it is not surprising that chromatograms of SPMDs generally have higher amounts
of lower KOW or more water-soluble compounds.
Also, biota more readily
metabolize or depurate most low KOW compounds.
Finally, if one allows sufficient exposure time for SPMDs to approach
equilibrium for all accumulated compounds, differences between the
chromatographic profiles of low KOW and high KOW chemicals
(sampled earlier) should be reduced.
Because many types of
environmental stressors can affect the health, and thus the dietary and
respiratory uptake of chemicals by transplanted biomonitoring organisms, a
disparity may exist between the number and relative amounts of analyte residues
detected in SPMDs and the tissues of test animals.
The following figure illustrates this difficulty.
This side-by-side
exposure of SPMDs and clams shows that the number and amounts of chemicals
accumulated by SPMDs and biomonitoring organisms are not always comparable.
In the case shown above, clams accumulated only a small fraction of the
PAHs residues concentrated by the SPMDs. The
investigators (Moring and Rose, 1997) suggested that the clams were not
filtering water (feeding) during most of the exposure, because of stress.
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Use of certain in vitro
biomarker/bioindicator assay to assess ecosystem health is sometimes
problematic, because of the difficulty of obtaining samples suitable for
testing. Most hydrophobic organic
contaminants are present in environmental water only at trace levels (i.e., <
1 µg/L). However, the
sometimes-slow process of bioconcentration (uptake from water, respiratory and
dermal absorption [e.g., non-scaled fish])/bioaccumulation (dietary,
respiratory, and dermal absorptive uptake) can lead to elevated concentrations
of contaminants in aquatic organism tissues, which can result in a variety of
adverse effects. In some cases,
samples and procedures used for cellular-based assays may not account for the
potential effects of bioconcentration. Also,
some bioindicator tests have relatively low sensitivities for many pollutants.
Thus, direct testing of environmental waters with these assays may lead
to false-negative errors in assessing the potential risk of waterborne residues
to aquatic life. To avoid this type
of error and expand the use of these tests for ranking toxicity potential, a
preconcentration method is often needed that mimics the biouptake process.
Complex mixtures of
chemicals are mimetically sequestered by SPMDs and are often amenable to
examination by a variety of bioassays. These
assays include both biomarker/bioindicator tests and immunoassays.
Assays that have been used to assess SPMD extracts or diluents include
the following: Microtox®, Mutatox®, mixed-function oxygenase induction-ethoxyresorufin-o-deethylase
(EROD) activity, sister chromatid exchange, vitellogenin induction via
interperitoneal injection of test species, enzyme-linked immunosorbent assay,
and Ames mutagenicity test (note that this list is not all inclusive).
The marriage of SPMDs and compatible biomarker/bioindicator tests offers
many avenues of investigation, all potentially providing information concerning
the relative toxicological significance of chemicals present in the
environmental matrices sampled.
However, two issues should
be considered to ensure that the results of SPMD-biomarker/bioindicator tests
provide toxicologically relevant information.
First, the level of residue preconcentration by the SPMD should be less
or fall within a range of estimated bioconcentration/bioaccumulation levels in
feral organism tissues. Secondly,
the levels of oleic acid and elemental sulfur in SPMD extracts should be kept at
a minimum. Fatty acids are known to
be cytotoxic and sulfur may be reduced to toxic sulfides (Brouwer and Murphy,
1995). The toxicity of fatty acids
such as oleic acid has been attributed to their membrane disturbing properties,
which include disruption of the calcium pump by the formation of metal salts (Sabaliunas
et al., 2001). Oleic acid is the
only fatty acid present as an impurity in the 95% triolein commonly used in
SPMDs. During environmental
exposures, a significant portion of this triolein impurity diffuses to the
exterior surface of an SPMD, where dissipation and/or degradation occur.
Unfortunately no or little attenuation occurs in the oleic acid levels in
laboratory SPMD-field blanks, -fabrication blanks and -process blanks.
Thus, the potential for significant differences in biomarker/bioindicator
test responses exist among reference site (i.e., no toxicant present) exposed
SPMDs and associated field and laboratory QC SPMD samples. Fortunately, only extremely low levels of oleic acid are
present in some commercially available triolein (e.g., Sigma, 99 %, and Nu-Chek
Prep., Inc., 99 %). If cost limitations require the use of triolein with oleic
acid, a simple silica gel cleanup step can be used to separate oleic acid from
target pollutants in SPMD extracts (contact Jon Lebo, CERC, USGS, Columbia, MO,
USA, ph: 573-876-1837) and may be scaled up to purify triolein prior to use in
SPMDs. Also, it is noteworthy that
fatty acids are commonly present in extracts of fish and other aquatic
organisms. In the case of sulfur, many types of sediment contain relatively
large amounts of elemental sulfur and elemental sulfur is readily accumulated by
SPMDs. To ensure that the results
of biomarker/bioindicator tests reflect the effects of target compounds,
elemental sulfur can be removed from extracts by treatment with size exclusion
chromatography or with shiny copper (contact Jon Lebo, CERC, USGS, Columbia, MO,
USA, ph: 573-876-1837).
The following figure and
table illustrate the application of SPMDs as mimetic sample
concentration/collection devices:
Use
of Microtox® and Mutatox® to Determine the Toxicity of
SPMD Concentratesa. Microtox
values are 5-minute EC-50s with 95% confidence intervals (in parentheses);
Mutatox values show positive response as "+" and negative response as
"-" (courtesy of Tom Johnson).
Sample Type |
Microtox Toxicity (EC-50)a |
Mutatox Genotoxicity (+/-) |
SPMDs |
|
|
Winter Quarters Bayb |
3.1 |
- |
McMurdo Soundb |
88 |
- |
Flat Branchc |
NAd |
+ |
Quality Control |
|
|
Procedural Blanke |
NDf |
- |
SPMD Controlg |
ND |
- |
Microtox phenol reference toxicant (µg/mL H2O) |
19 |
NA |
Mutatox
benzo-a-pyrene reference toxicant (1.0 µg/vial) |
NA |
+ |
a
Assays were
conducted on lipid diluent or dialysates and EC-50 values represent mg SPMD
lipid/mL carrier solvent
b
SPMDs were
exposed to Antarctica sediments in microcosms
c SPMDs were exposed to a small urban stream
d None analyzed
e Solvents/reagents used in tests
f None detected
g Freshly prepared SPMD; carried through Microtox and Mutatox test
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The figure shown below
demonstrates that PCB vapors (top chromatogram) are readily sampled by SPMDs.
In fact, the potential utility of SPMDs for atmospheric sampling (e.g.,
Petty et al., 1993 and Ockenden et al., 1998) is as great as that of water.
In general, the linear uptake rates (i.e., volumetric Rss and
kus) are about a thousand times higher in air than in water. The much larger volumes of air sampled, relative to water,
are primarily due to the approximately 10³ higher diffusion coefficients of
vapors relative to aqueous solutes. However,
when the difference in the density of water and air is considered, the adjusted
sampling rates for the two phases are of similar magnitude.
Note that we evoke differences in media density solely for comparative
purposes, as density corrections are not performed in interphase mass transfer
models.
There is little
calibration data (standard SPMD sampling rates) in the literature other than
those of Ockenden et al., 1998. The
results of the Ockenden et al., 1998 and unpublished work by CERC scientist,
indicated that for a wide range of PCB KOWs
(exposure condition: low air velocity at 4 °C
to 26 °C), the Rss for standard SPMDs varied from
about 0.5 m³/d to 20 m³/d. Currently,
additional calibration studies are underway at CERC.
Similar to water, the rate-limiting step in the uptake of hydrophobic
chemicals may be the external boundary layer, because the "effective"
mass-transfer resistance in the membrane is less in the air than in water, as
values of a chemical's KOA are generally much higher than it's KOW.
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The table below shows that
SPMDs sample sediment associated contaminant residues. Exposure conditions in the bed sediments of many aquatic
environments are less variable than in the water column.
Therefore, the sometimes-large differences in the sampling rate of a
target compound in the water column at different sites (largely due to changes
in hydrodynamics) should not materialize in bed sediments.
On the other hand, the heterogeneity of the amount and quality of
sediment organic carbon and textural differences at sample sites likely plays a
major role in the amount of chemical accumulated in SPMDs.
When using SPMDs to sample
the water column of aquatic systems, chemical concentrations in the outer
portion of the device’s aqueous boundary layer reflect residue levels in the
bulk medium, because of rapid mixing-exchange of residues from the water column.
In the case of SPMDs placed in sediments, resupply of hydrophobic
residues extracted from the SPMD-associated aqueous boundary layer and/or
contiguous pore water may be limited by the rate of residue desorption from
sediment particles and/or slow diffusion in stagnant pore water and in sediment
organic matter. Comparison of chemical concentration factors (CFs) in the
triolein (i.e., residue concentration in SPMD lipid divided by the residue
concentration in the water column just above the sediment) of SPMDs covered by
sediments to those measured in SPMDs placed in slowly flowing water free of
sediments (similar temperatures) showed that the CFs in sediment-exposed SPMDs
were about half of those observed for SPMDs exposed in water alone (see table
below for CFs of selected compounds in SPMDs in sediment).
Note that this potential discrepancy should disappear if actual
pore-water concentrations were known. This
data suggests that the concentration of 2, 2', 5, 5'-TCB in porewater contiguous
to the SPMD was significantly reduced relative to the water column. In general, the concentrations of chemicals in relatively
undisturbed pore water of benthic sediments are expected to be greater than the
concentrations of the same compounds in the water column.
Until SPMDs reach equilibrium with contiguous sediments, estimation of
the "undisturbed" porewater concentrations of high KOW
compounds is not possible. However,
use of solid phase microextraction (SPMEs) fibers with very thin films (e.g., 7
µm film thickness of polydimethysiloxane [PDMS]) of sorbent may permit
estimation of non-disturbed pore water concentrations.
These thin-film SPMEs have high surface area for solute exchange and
low-sorbent volume, which reduce the time required toe reach equilibrium with
sediment-associated residues. Once
equilibrium is achieved, computation of undisturbed pore water concentrations is
straightforward.
Although SPMDs generally will not reach equilibrium with pore water, they provide valuable information on the amount of bioconcentratable residues available during a window of time. Perhaps the best approach for the characterization of contaminated sediments is a two-part assessment, where SPMDs are used in situ to measure the flux of bioavailable chemicals (results relate to the toxicity of sediments to laboratory test organisms), and to detect and collect relatively large amounts of trace-level bioavailable contaminants (may be used for bioassay or toxicity identification evaluation procedures).
Exposure
of SPMDs1 to Contaminated Sediment2
|
Concentration
Factor (CF) in Triolein |
|||
Analyte |
1 day |
7 days |
14 days |
28 days |
Phenanthrene |
2,380 |
14,600 |
7,800 |
42,500 |
Dieldrin |
350 |
4,740 |
6,540 |
10,940 |
2, 2', 5, 5'-TCB 3 |
2,650 |
13,000 |
26,600 |
38,800 |
1
SPMDs (n = 3/test chemical) contained 0.1 g triolein and were covered by
sediment
2 300-g sediment (% organic = 1%) and 950 mL CERC well water
3 Tetrachlorobiphenyl
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The table below shows that
SPMDs and aquatic organisms often have similar uptakes rates (kus)
for hydrophobic organic chemicals, but the clearance rates (kes and t1/2s)
of accumulated residues from organisms are generally much faster than SPMDs (see
table below and the two related figures that follow).
Remember that integrative sampling requires that sampling is additive
through time, i.e., once residues are taken up they are not lost when
environmental concentrations vary. The observed difference in the residence
times of residues in the two matrices is due to several factors.
Only relatively slow, surface area dependent, passive diffusive exchange
processes govern the rates of residue losses from SPMDs, whereas residue-loss
rates from aquatic organisms are governed by much more complex processes.
Active respiration, feeding, waste elimination, metabolism, reproduction
(females) and passive diffusion combine to control the depuration of accumulated
contaminant residues from organisms. Obviously, another major difference between SPMDs and nearly all
aquatic organisms is that SPMDs have a much larger lipid pool than organisms of
equivalent mass and, unlike organism proteins, the LDPE membrane significantly
adds to the capacity of the sampler.
Comparison
of SPMD and Organism Uptake (ku) And Clearance (ke) Rate
Constants
for Selected Chemicals
CHEMICAL |
SPMD
(membrane
+ lipid) ku(Ld-1g-1) ke(t-1) t1/2* |
ku(Ld-1g-1) ke(t-1) t1/2 |
||||
naphthalenea |
0.15 |
0.0220 |
32 h |
0.20 0.08 |
1.6670 (Daphnia pulex) 0.1990 (fish) |
0.4 h 3.5 h |
acenaphthaleneb |
0.42 |
0.0029 |
240 h |
- |
- |
- |
phenanthrenec |
0.63 |
0.0014 |
500 h |
0.20 |
0.5430 (Daphnia pulex) |
1.3 h |
2, 2', 5-trichlorobiphenyld |
2.24 |
- |
- |
1.20 0.95 |
- (Brown Trout) 0.0480 (Goldfish) |
- 346 h |
2, 2', 5, 5'-tetrachlorobiphenyle |
1.82 |
0.0004 |
1,730 h |
1.40 - |
- (Brown Trout) 0.0016 (Zebra Fish) |
- 433 h |
a
SPMD: This work; MacKay et al., 1992, organism not specified
b SPMD: This work
c
SPMD: This work;
Biota, MacKay et al., 1992
d SPMD & Trout: Meadows, CERC, 1996;Goldfish, MacKay, et al.,
1992
e SPMD & Trout: Meadows, CERC, 1996; Zebra Fish, MacKay, et al.,
1992
* First-order half-lives
The much longer half-lives
and kes shown in the table above indicate that SPMDs are better
suited for integrative sampling of contaminant residues.
The passive integrative sampling of high KOW compounds by
SPMDs enables detection of episodic releases and provides more accurate time
weighted average estimates of water concentrations.
On the other hand, biomonitoring organisms are more likely to reach
steady state concentrations, may sample ionic compounds (unlike SPMDs), and the
analysis of feral organisms is essential for determining residue concentrations
in edible tissues. However, residue
concentrations in biomonitoring organism tissues often may not be proportional
to ambient environmental concentrations of contaminants, which suggest that
tissues levels cannot reliably be used to derive water concentrations and thus
differences in bioavailable pollutant levels at study sites may often be
difficult to discern.
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Comparisons of SPMDs and Biota (Kinetics and Steady
State)
Requirements for Lipid Normalization:
|
·
Samples
must be at steady state or equilibrium with ambient environment (seldom
the case with SPMDs) |
|
·
Solvents
and methods used for sample extraction must be similar to ensure recovery
of the same types and amounts of sample lipid |
Assumptions of Lipid Normalization:
|
·
Differences
in lipid composition among individuals and species have little or no
effect on the magnitude of equilibrium lipid/water partition coefficient |
|
·
Variance
is decreased relative to non-normalized data |
Conclusion:
Lipid normalization is
often inappropriate, especially in the case of SPMD-biota
comparisons, largely because SPMDs seldom reach steady-state concentrations.
Although this tutorial
covers many of the key elements of SPMD technology, it is not comprehensive and
certain aspects will be updated as ongoing research is completed.
The annual or semiannual International SPMD Workshops are excellent
sources of information on current developments in SPMD technology.
(Contact Environmental Sampling Technologies, 1717 Commercial Drive, St.
Joseph, MO 64503.)
If the reader has additional questions concerning SPMDs, contact Dave Alvarez: (573) 441-2970; e-mail: dalvarez@usgs.gov
We have also prepared
answers to 20 frequently asked questions (FAQs)
related to SPMD technology.
See References
for peer-reviewed journal articles about various aspects of Semipermeable
Membrane Devices and their applications and for articles referred to in the
tutorial. Also, the reader should
be aware of an extensive forthcoming report for the American Petroleum Institute
(API): "Guide for the Use of SPMDs as Samplers of Waterborne
Hydrophobic Organic Contaminants," API no. 4690, In Press.
This document expands the discussions herein, provides an extensive set
of calibration data for standard SPMDs, and covers topics not discussed in this
tutorial.
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