photo-induced toxicity of deepwater horizon spill oil to .../67531/metadc822778/m2/1/high_res... ·...
TRANSCRIPT
PHOTO-INDUCED TOXICITY OF DEEPWATER HORIZON SPILL OIL TO FOUR NATIVE
GULF OF MEXICO SPECIES
Matthew M. Alloy
Dissertation Prepared for the Degree of
DOCTOR OF PHILOSOPHY
UNIVERSITY OF NORTH TEXAS
December 2015
Approved By:
Aaron Roberts, Major Professor
Samuel Atkinson, Committee Member
Barney Venables, Committee Member
James Oris, Committee Member
James Stoeckel, Committee Member
Alloy, Matthew M. Photo-Induced Toxicity of Deepwater Horizon Spill Oil to Four Native
Gulf of Mexico Species. Doctor of Philosophy (Environmental Science), December 2015, 88 pp.,
references, 212 titles.
The 2010 Deepwater Horizon oil spill resulted in the accidental release of millions of
barrels of crude oil into the Gulf of Mexico (GoM). Photo-induced toxicity following co-exposure
to ultraviolet (UV) radiation is one mechanism by which polycyclic aromatic hydrocarbons
(PAHs) from oil spills may exert toxicity. Blue crab (Callinectes sapidus) are an important
commercial and ecological resource in the Gulf of Mexico and their largely transparent larvae
may make them sensitive to PAH photo-induced toxicity. Mahi-mahi (Coryphaena hippurus), an
important fishery resource, have positively buoyant, transparent eggs. These characteristics
may result in mahi-mahi embryos being at particular risk from photo-induced toxicity. Red
drum (Sciaenops ocellatus) and speckled seatrout (Cynoscion nebulosus) are both important
fishery resources in the GoM. They spawn near-shore and produce positively buoyant embryos
that hatch into larvae in about 24 h. The goal of this body of work was to determine whether
exposure to UV as natural sunlight enhances the toxicity of crude oil to early lifestage GoM
species. Larval and embryonic organisms were exposed to several dilutions of water
accommodated fractions (WAF) from several different oils collected in the field under chain of
custody during the 2010 spill and two to three gradations of natural sunlight in a factorial
design. Here, we report that co-exposure to natural sunlight and oil significantly reduced larval
survival and embryo hatch compared to exposure to oil alone.
iii
TABLE OF CONTENTS
Chapters
1. INTRODUCTION 1
Polycyclic Aromatic Hydrocarbons 1
Photo-induced Toxicity 2
Factors Influencing Photo-induced Toxicity 5
Photo-induced Toxicity and Oil 6
Deepwater Horizon Spill 8
References 11
2. PHOTO–INDUCED TOXICITY OF DEEPWATER HORIZON SLICK OIL TO BLUE CRAB
(CALLINECTES SAPIDUS) LARVAE 18
Introduction 19
Methods 19
Test Organism 19
Test Solutions 19
Toxicity Tests 21
Phototoxic Units 22
Statistical Analyses 23
Results 24
Toxicity Associated with WAF Preparation 24
Toxicity Associated with Oil Source 25
Discussion 30
Acknowledgements 33
References 34
3. ULTRAVIOLET RADIATION ENHANCES THE TOXICITY OF DEEPWATER HORIZON OIL TO
MAHI MAHI (CORYPHAENA HIPPURUS) EMBRYOS 37
Introduction 37
Materials and Methods 38
iv
Test Organism 38
Test Solutions 39
Toxicity Tests 40
Phototoxic Units 41
Statistical Analyses 42
Results 42
Discussion 47
Toxicity Associated with WAF Preparation Method 48
Toxicity Associated with Oil Source 49
Acknowledgements 52
References 53
4. SENSITIVITY OF EARLY LIFESTAGE RED DRUM (SCIAENOPS OCELLATUS) AND SPECKLED
SEATROUT (CYNOSCION NEBULOSUS) TO PHOTO–INDUCED TOXICITY OF NATURALLY
WEATHERED DEEPWATER HORIZON OIL 57
Introduction 57
Materials and Methods 59
Test Organisms 59
Test Solutions 59
Toxicity Tests 60
Phototoxic Units 61
Statistical Analyses 62
Results 62
Discussion 69
Acknowledgements 71
References 72
5. DISCUSSION 77
v
Influences on Polycyclic Aromatic Hydrocarbon Tissue Concentrations 77
Ultraviolet Wavelength Absorbing Pigmentation 80
Factors Relating to Species Sensitivity 82
Possible Effects on Recruitment 84
Acknowledgements 86
References 87
1
INTRODUCTION
Polycyclic Aromatic Hydrocarbons
Polycyclic aromatic hydrocarbons (PAHs) are a broad classification of environmental
contaminants. They consist of organic molecules with multiple ring structures and vary widely
in their chemical and toxicological properties [1, 2]. PAHs are rarely found in the environment
as a single chemical species. Typically, they are a complex mixture with a wide variety of
environmental sources including: geological seepage, industrial processing, combustion engine
operation and lubrication, volcanic activity, natural and anthropogenic fires, accidental release
from oil and coal extraction and transport [3].
The individual properties of PAHs vary widely. The two-ring PAH napthalene has a
molecular weight of 128.2 g/mol and a logkow of 3.37, while the five-ring PAH benzo[a]pyrene
has a molecular weight of 252 g/mol and a logkow of 6.04 [4]. The variety of characteristics of
PAHs means that they cover a fairly broad range of chemical and biological actions. They range
from volatile to relatively non-volatile and moderately hydrophobic to highly hydrophobic [4].
In a mixed PAH release, such as crude oil seep or spills, not all constituents of the mixture will
share the same environmental fate. PAHs associated with surface water can volatilize, oxidize,
photolyze, or biodegrade [5]. On the surface the volatiles will tend to diffuse to the gaseous
phase according to Henry’s Law [5, 6] leaving the less volatile fraction to undergo physical
weathering and possible dissolution into the water. They can also partition from the aqueous
phase to associate with sediments or be absorbed into biota [7]. Uptake of PAHs from
sediments or water into the organism differs among species. Exposure routes leading to uptake
2
take the form of ingestion or diffusion based on the difference in hydrophobicity between the
organism and the aqueous environment [7]. Ingestion of PAHs can be from the food item’s
body burden, or incidental as with the ingestion of sediment particles during the course of
feeding. Diffusion is thought to be primarily across the gill surfaces during respiratory activity,
but it may also occur across the organism’s integument [8, 9]. PAHs above the surface of the
water or above the UV extinction depth will also be subject to UV photolysis [4, 10]. This can
create various breakdown products by itself [5], and bacterial metabolism can create others
[11].
Despite the variety in PAH characteristics and distributions, PAHs hold some modes of
toxicity in common, most notably by narcosis in aquatic organisms [12]. Narcosis is caused by
the partitioning of hydrophobic PAHs into the cell membranes of neuron tissues, depressing
central nervous system activity [13, 14]. Any PAH without functional groups and two to four
rings can have a narcotic effect on fish [15]. PAHs have been known to cause developmental
defects in larval organisms, specifically; cardiac malformation [16-20], craniofacial defects,
spinal-axis defects [21] ocular malformations [23], and neurodevelopmental defects [24]. It has
also been observed that fish immune system function can be depressed by PAHs [25, 26]. The
current model for the teratogenesis of PAHs is the activation of the Aryl Hydrocarbon receptor
by PAHs during key stages of development interferes with normal developmental regulation
[27-30].
Photo-induced Toxicity
Photo-induced toxicity is the phenomenon of a co-exposure of light increasing the
toxicity of a compound. Sometimes this increase can be more than a thousand fold [31-33]. It
3
can occur broadly across kingdoms, in plants [34-36], and in animals [18, 37-51]. Compounds
that exhibit photo-induced toxicity vary across classifications, from pesticides, to endogenous
phytochemicals, and PAHs [33].
Photo-induced toxicity can refer to two classes of mechanisms, photosensitizers, and
photomodified toxicants. A photosensitizer is a molecule that, after cellular uptake, can cause
damage to cell membranes, enzymes, organelles, and DNA by generation of reactive oxygen
species (ROS) in the presence of UV light of a specific wavelength range. A photomodified
compound is one that has been altered in structure by UV light, enhancing its toxicity relative to
the parent compound. Often these are quinones. Modification can occur immediately prior to,
or even a relatively long time before exposure to the target organism. Pre-irradiation of a PAH
subject to photomodification prior to exposure to organisms will increase observed toxicity [52]
while photosensitizers require simultaneous exposure to UV and PAH. For example,
phenanthrene can photooxidize to 9,10-phenanthrenequinone, anthracene can become
anthraquinone or dihydroxyanthraquinone, and benzo[a]pyrene can become
phenanthrenequione, or benzo[a]pyrenequinone [10]. In the case of a metal bound to an
organic compound, photoreaction can release the metal, making it bioavailable which could
result in toxic effects [53, 54].
The mechanism of action for photosensitizers is the production of ROS by the
absorption of certain wavelengths of light [55]. All wavelengths of light travel at the same rate
of propagation based upon the media traveled through. Velocity is held constant, variation in
wavelength is then determined by the energy of the photons. Therefore, the shorter the
wavelength, the more energy the photon has. UV radiation consists of wavelengths between
4
100nm and 400nm. The wavelengths of UV that are primarily responsible for photosensitization
reactions are between 320nm and 400nm, the absorbance range for UV for most PAHs [55].
Photosensitization occurs when a photodynamic PAH is absorbed by an organism which
is then subsequently exposed to ultraviolet radiation. This radiation must penetrate the cell to
reach the PAH and be of a wavelength that, once absorbed by the PAH molecule, excites an
electron to jump the gap from the PAH’s highest occupied orbital to the lowest unoccupied
orbital (HOMO-LUMO gap) [56]. This excited state is then often resolved by reaction with
dissolved oxygen to form an oxygen radical. Damage to cell structures most often results from
this oxygen radical starting a lipid peroxidation chain reaction. This action is dependent on the
wavelength/intensity of the UV exposure matching the HOMO-LUMO gap of the
photosensitizer in question. The wider the HOMO-LUMO gap, the less often an excited electron
will be able to achieve sufficient excitation to initiate a Type I or II reaction [33]. HOMO-LUMO
gap width has been used successfully to group PAHs into potentially phototoxic and non-
phototoxic [2, 57]. Once in the singlet excited state, the photosensitizer can react with
molecular oxygen or another receptive molecule or the electron can lose the gained energy by
thermal emission, fluorescence, or conversion to a triplet state (Figure 1). If the excited electron
is passed to a biological molecule it is known as a Type I reaction. If the singlet or triplet state
reacts with molecular oxygen it is known as a Type II reaction [58]. In the case of a Type I
reaction, the recipient molecule typically responsible for observed cellular damage is a lipid,
forming lipid peroxides that can result in cellular membrane damage leading to cell death [59].
In the case of a Type II reaction, singlet oxygen becomes an intermediary step towards reaction
with biomolecules to ultimately produce the same ROS damaging effects on organelles and
5
membranes [60, 61]. This damage on a tissue level can result in reduced function of an organ,
such as increased oxygen diffusion distance and reduced osmoregularity in the gill [62, 63].
Damage by an intermediary oxidation step or by direct oxidative damage to DNA can lead to
DNA adduct formation, and single strand breaks [2, 64]. It has also been demonstrated in the
literature that established PAH carcinogenicity can be enhanced by photo-activation [2]. Whole
organism effects that have been reported in the literature include: reduction in organism
fecundity [43], photo-avoidance behaviors [65], and feeding inhibition [66].
Figure 1. Photo-excitation leading to either a singlet state and reaction or a triplet state and a reaction.
Factors Influencing Photo-induced Toxicity
Incident solar radiation of any given location is dependent on several variables. The
latitude and season determine the base intensity of solar radiation prior to atmospheric
attenuation [67, 68]. Latitude also affects atmospheric attenuation. The angle of incidence close
to the equator presents less atmospheric gases to attenuate UV. At higher latitudes the angle of
6
incidence can almost double the effective thickness of the atmosphere, resulting in greater
attenuation of UV prior to reaching surface waters [69]. The thickness of the stratospheric
ozone layer is a strong determinant of small wavelength UV radiation. The majority of high
energy UVC (100nm to 280nm) is removed by the ozone layer. Lower energy ranges, UVB
(280nm to 315nm) and UVA (315nm to 400nm), are attenuated to a lesser degree before
reaching surface waters [70]. Many factors determine the depth of UV extinction including
intensity of incident UV at the surface and water column characteristics such as suspended
solids, dissolved organic carbon (DOC), and salinity [70]. The composition of the dissolved and
suspended components in the water can affect which wavelengths are most efficiently
screened out and what rate per unit depth [44, 70-73]. This wavelength specific screening can
shift potential for photosensitized toxicity by reducing the available energy needed for
photomodification or for its HOMO-LUMO gap. The degree to which dissolved organic carbon
has been photobleached also influences the UV in the system. Photobleached DOC fails to
attenuate as much UV as the same concentration of unbleached DOC [73]. Some forms of DOC
can influence photo-induced toxicity in other ways; Oris et al. [44] showed that humic acids can
reduce the bioaccumulation factor of PAHs in addition to UV attenuation. Salinity in systems
has been linked to greater UV penetrance in systems [70, 71]. Weinstein [74] reported that
salinity influenced PAH bioaccumulation and photo-induced toxicity in one estuarine species,
but not another. Weinstein concluded that the organism’s osmoregulation strategy was what
determined whether salinity could influence PAH bioaccumulation.
Photo-induced Toxicity and Oil
7
Photo-induced toxicity caused by PAHs has been reported in the literature in both the
laboratory and in situ. Calfee et al. [40] reported phototoxic effects in Daphina when exposed
to the water accommodated fraction (WAF) of oil collected from an abandoned offshore oil
field. Cleveland et al. [41] reported phototoxic effects to Mysid shrimp exposed to WAF from a
Guadalupe oil field. Ireland et al. [75] conducted a test between an upstream reference site and
a PAH contaminated section of river; the authors reported lethal photo-induced toxicity in
Daphnia in their field study as well as in a chronic laboratory assay. Little et al. [76] tested
underground free plume oil acquired under an abandoned oil field for photo-induced toxicity
using indoor solar simulators to tidewater silverside fish, and reported an order of magnitude
lower LC50s for their UV treatment compared to treatments lacking UV irradiation. Monson et
al. [77] investigated phototoxic effects on nematodes in PAH contaminated sediments, both in
the field and in control environments. The authors reported significant mortality in all
treatments where the test organisms were co-exposed to UV light and PAHs, and less than
twenty percent mortality all PAH treatments without UV light exposure. Peachey and Crosby
[78] performed PAH photo-induced toxicity assays on five different phyla of marine organisms
which inhabit reef flats known to have intense UV exposure. Among PAH exposures ranging
from 0 µg /L to 48 µg/L they reported four species which displayed no adverse effect with co-
exposure to UV and PAH, five species that displayed various toxic response within the tested
range and two species which displayed great sensitivity to co-exposure.
Part of the complexity of PAH toxicity is the tendency for PAH mixtures to change in
composition once released into aquatic systems. Photolysis, and bacterial metabolism can alter
toxicity of individual PAH compounds. This weathering effect has been tested and reported in
8
the literature to have increased phototoxic effect. Maki et al. [79] biodegraded Arabian crude
oil for 21 days, then exposed the degraded oil to solar irradiation for up to twenty-eight days.
The authors used this biodegraded and photo degraded oil to investigate photo-induced
toxicity to artemia napulii. They reported photo-induced toxicity to artemia exposed to WAF for
twenty-four hours increased as the solar weathering pretreatment period increased, exhibiting
the greatest toxicity at twenty-five days of irradiation. Environmental factors such as
temperature, pH, and dissolved oxygen can influence the rate of PAH photolysis [80]. The same
study concluded that photolysis rates in PAHs with four rings or more are influenced by pH and
dissolved oxygen. PAHs with fewer than four rings have photolysis rates independent of pH and
dissolved oxygen. Simulated solar weathering of Brazilian crude oil for sixty-four hours resulted
in decreases in the aliphatic and aromatic fractions, and an increase in the polar fraction of the
oil mixture [81]. Composition of PAHs in various crude oil sources is not homogenous, and oils
from different sources may weather differently [82].
The PAHs observed to be in Exxon-Valdez spill water included known photosensitizers
[15]. Ultraviolet light has been shown to penetrate as deeply as 25 meters in Port Valdez waters
under good conditions, and 6 meters even under turbid conditions [15]. Duesterloh et al. [83]
tested the photo-induced toxicity of weathered North Slope Alaskan crude oil to two species of
calanoid copepods. The authors exposed their test organisms to oil concentrations of 2 µg/L,
and two UVA treatments, high UVA (14,253 µW/cm2 total dose), low UVA (6,202 µW/cm2 total
dose), and a no-UVA treatment. They reported significant affects to both test organisms in all
UVA + oil co-exposures relative to oil only exposures.
Deepwater Horizon Spill
9
Beginning on the 20th of April, 2010, the Mobile Offshore Drilling Unit Deepwater
Horizon experienced a series of events that resulted in the sinking of the vessel and subsequent
oil release from the wellhead. On the 15th of July the oil release was controlled, and the
wellhead declared safe on the 19th of September, 2010. Over the period of uncontrolled oil
release –87 days in length– millions of barrels of oil was released [84].
Subsurface oil monitoring was conducted by various groups to monitor the amount of
oil release that was not reaching surface waters. PAH analysis of water samples taken at known
depth and locations indicated several subsurface plumes existed, some for months without
significant degradation, the largest of which was found at approximately 1,100 meters in depth
and to be in a continuous layer for 35 kilometers with a benzene, toluene, ethylbenzene, and
xylenes (BTEX) concentrations as high as 78 µg/L [85].
Approximately 25.5 thousand barrels of dispersants were utilized over the course of the
87 day oil spill [86]. The dispersants were not totally successful in the goal of preventing oil
from reaching the surface (Figure 2). Kujawinski et al. [87] reported that biota encountering
plumes within 10 kilometers of the wellhead might have been exposed to dispersant
concentrations within the range of 10 µg/L to 100 µg/L. They also reported measuring dioctyl
sodium sulfosuccinate (DOSS) –a component in both Corexit 9527 and 9500A formulations used
on the spill– in nanogram per liter concentrations in some sample sites as far as 300 kilometers
from the well head.
11
References
1. Ankley GT, Burkhard LP, Cook PM, Diamond SA, Erickson RJ, Mount DR. 2003. Assessing
Risks from Photoactivated Toxicity of PAHs to Aquatic Organisms. Douben PET Ed. PAHs:
An Ecological Perspective, John Wiley & Sons Ltd. West Sussex, England. pp 273-296.
2. Arfsten DP, Schaeffer DJ, Mulveny DC. 1996. The effects of near ultraviolet radiation on
the toxic effects of polycyclic aromatic hydrocarbons in animals and plants: a review.
Ecotoxicol. Environ. Saf. 33: 1-24.
3. Durieux EDH, Connon RE, Werner I, D’Abronzo LS, Fitzgerald PS, Spearow JL, Ostrach DJ.
2012. Cytochrome P4501A mRNA and protein induction in striped bass (Morone
saxatilis). Fish Physiol Biochem. 38: 1107-1116.
4. Latimer JS, Zheng J. 2003 The sources, transport, and fate of PAHs in the marine
environment. Douben PET Ed. PAHs: An Ecological Perspective, John Wiley & Sons Ltd.
West Sussex, England. pp 7-33.
5. Aeppli C, Carmichael CA, Nelson RK, Lemkau KL, Graham WM, Redmond MC, Valentine
DL, Reddy CM. 2012. Oil Weathering after the Deepwater Horizon Disaster Led to the
Formation of Oxygenated Residues. Environ. Sci. Chem. 46: 8799-8807.
6. Bamford HA, Poster DL, Baker JE. 1999. Temperature dependence of Henry’s Law
constants of thirteen polycyclic aromatic hydrocarbons between 4°C and 31°C. Environ.
Toxicol. Chem. 18: 1905-1912.
7. Meador JP. 2003. Bioaccumulation of PAHs in marine invertebrates. Douben PET Ed.
PAHs: An Ecological Perspective, John Wiley & Sons Ltd. West Sussex, England. pp 147-
171.
8. Landrum PF, Stubblefield CR. 1991. Role of respiration in the accumulation of organic
xenobiotics by the amphipod Diporeia sp. Environ. Toxicol. Chem. 10: 1019-1028.
9. Willis AM, Oris JT. 2014. Acute photo-induced toxicity and toxicokinetics of single
compounds and mixtures of polycyclic aromatic hydrocarbons in zebrafish. Environ.
Toxicol. Chem. 33(9): 2028-2037.
10. McConkey BJ, Duxbury CL, Dixon DG, Greenburg, BM. 1997. Toxicity of a PAH
Photooxidation Product to the Bacteria Photobacterium phosphoreum and the
Duckweed Lemna gibba: Effects of the Phenanthrene and its Primary Photoproduct,
Phenanthrenequinone. Environ. Tox. Chem. 16(5): 892-899.
11. Cerniglia CE. 1993. Biodegradation of polycyclic aromatic hydrocarbons. Curr Opin
Biotech. 4: 331-338.
12. Lee JH, Landrum PF, Koh CH. 2002. Toxicokinetics and time-dependent PAH toxicity in
the amphipod Hyalella azteca. Environ. Sci. Technol. 36: 3124-3130.
13. Barron MG. 2002. Environmental contaminants altering behavior. Dell’Omo G, ed. Behav
ecotoxicol, John Wiley and Sons Ltd, New York, pp 167-186.
12
14. Verhaar HJM, De Wolf W, Dyer S, Legierse KCHM, Seinen W, Hermens JLM. 1999. An
LC50 vs Time Model for the Aquatic Toxicity of Reactive and Receptor-Mediated
Compounds. Consequences for Bioconcentration Kinetics and Risk Assessment. Environ.
Sci. Technol. 33: 758-763.
15. Barron MG, Ka'aihue L. 2001. Potential for photoenhanced toxicity of spilled oil in Prince
William Sound and Gulf of Alaska waters. Mar. Pollut. Bull. 43(1): 86-92.
16. Mager EM, Esbaugh AJ, Stieglitz JD, Hoenig R, Bodinier, C, Incardona JP, Scholz NL,
Benetti DD, Grosell M. 2014. Acute embryonic or juvenile exposure to Deepwater
Horizon crude oil impairs the swimming performance of mahi-mahi (Coryphaena
hippurus). Environ. Sci. Technol. 45(12): 7053-7061.
17. Incardona JP, Gardner LD, Linbo TL, Brown TL, Esbaugh AJ, Mager EM, Stieglitz JD,
French BL, Labenia JS, Laetz CA, Tagal M, Sloan CA, Elizur A, Benetti DD, Grosell M, Block
BA, Scholz NL. 2014. Deepwater Horizon crude oil impacts the developing hearts of large
predatory pelagic fish. Proc. Natl. Acad. Sci USA. 111(15): E1510-E1518.
18. Billard SM, Meyer JN, Wassenberg DM, Hodson PV, Di Giulio RT. 2008. Nonadditive
effects of PAHs on Early Vertebrate Development: Mechanisms and Implications for Risk
Assessment. Toxicol. Sci. 105(1): 5-23.
19. Perrichon P, Akcha F, Le Menach K, Goubeau M, Budzinski H, Cousin X, Bustamante P.
2015. Parental trophic exposure to three aromatic fractions of polycyclic aromatic
hydrocarbons in zebrafish: Consequences for the offspring. Sci Total Environ. 524: 52-62.
20. Huang L, Gao D, Zhang Y, Wang C, Zuo Z. 2014. Exposure to low dose benzo[a]pyrene
during early life stages causes symptoms similar to cardiac hypertrophy in adult
zebrafish. J Hazard Mater. 276: 377-382.
21. Incardona JP, Carls MG, Teraoka H, Sloan CA, Collier TK, Scholz NL. 2005. Aryl
hydrocarbon receptor-independent toxicity of weathered crude oil during fish
development. Environ. Heal. Persp. 113: 1755-1762.
22. Incardona JP, Swarts TL, Edmunds RC, Linbo TL, Aquilina-Beck A, Sloan CA, Gardner LD,
Block BA, Scholz NL. 2013. Exxon Valdez to Deepwater Horizon: Comparable toxicity of
both crude oils to fish early life stages. Aqua. Tox. 142: 303-316
23. Huang L, Wang C, Zhang Y, Wu M, Zou Z. 2013. Phenanthrene causes ocular
developmental toxicity in zebrafish embryos and the possible mechanisms involved. J
Hazard Mater. 261: 172-180.
24. He C, Wang C, Li B, Wu M, Geng H, Chen Y, Zuo Z. 2012. Exposure of Sebastscus
marmoratus embryos to pyrene results in neurodevelopmental defects and disturbs
related mechanisms. Aqua. Toxicol. 116: 109-115.
25. Reynaud S, Deschaux P. 2006. The effects of polycyclic aromatic hydrocarbons on the
immune system of fish: A review. Aqua. Toxicol. 77: 229-238.
13
26. Kim HN, Park C, Chae YS, Shim JW, Kim M, Addison RF, Jung J. 2013. Acute toxic
responses of the rockfish (Sebastes schlegeli) to Iranian heavy crude oil: Feeding disrupts
the biostransformation and innate immune systems. Fish Shellfish Immun. 35: 357-365.
27. Hahn ME. 2002. Aryl hydrocarbon receptors: diversity and evolution. Chem-Biol Interact.
141: 131-160.
28. Barouki R, Coumoul X, Fernandez-Salguero PM. 2007. The aryl hydrocarbon receptor,
more than a xenobiotic-interacting protein. FEBS Lett. 581: 3608-3615.
29. Mathew LK, Andreasen EA, Tanguay RL. 2006. Aryl Hydrocarbon Receptor Activation
Inhibits Regenerative Growth. Mol. Pharamacol. 69: 257-266.
30. Goodale BC, Tilton SC, Corvi MM, Wilson GR, Janszen DB, Anderson KA, Waters KM,
Tanguay RL. 2013. Structurally distinct polycyclic aromatic hydrocarbons induce
differential transcriptional responses in developing zebrafish. Toxico. App. Pharma. 272:
656-670.
31. Wernersson AS. 2003. Predicting petroleum phototoxicity. Ecotox. Environ. Safe. 54:
355-365.
32. Wernersson AS, Dave G. 1997. Phototoxicity Identification by Solid Phase Extraction and
Photoinduced Toxicity to Daphina magna. Arch. Environ. Contam. Toxicol. 32: 268-273.
33. Diamond SA, Milroy NJ, Mattson VR, Heinis LJ, Mount DR. 2003. Photoactivated toxicity
in amphipods collected from polycyclic aromatic hydrocarbon–contaminated
sites. Environ. Toxicol. Chem. 22(11): 2752-2760.
34. Ren L, Huang X, McConkey BJ, Dixon DG, Greenburg BM. 1994. Photoinduced Toxicity of
Three Polycyclic Aromatic Hydrocarbons (Fluoranthene, Pyrene, and Naphthalene) to
the Duckweed Lemna gibba. L. G-3. Ecotox. Environ. Safe. 28: 160-171.
35. Huang X, McConkey BJ, Babu TS, Greenburg BM. 1997. Mechanisms of Phototinduced
Toxicity of Photomodified Anthracene to Plants: Inhibition of Photosynthesis in the
Aquatic Higher Plant Lemna gibba (Duckweed). Environ. Toxicol. Chem. 16(8): 1707-
1715.
36. Gala WR, Giesy JP. 1992. Photo-Induced Toxicity of Anthracene to the Green Alga,
Selenastrum capricornutum. Environ. Contam. Toxicol. 23: 316-323.
37. Allred PM, Giesy JP. 1985. Solar Radiation-Induced Toxicity of Anthracene to Daphina
pulex. Environ. Toxicol. Chem. 4: 219-226.
38. Boese BL, Lamberson JO, Swartz RC, Ozretich RJ. 1997. Photoinduced toxicity of
fluoranthene to seven marine benthic crustaceans. Arch. Environ. Contam. Toxicol.
32(4): 389-393.
39. Bowling JW, Leversee GJ, Landrum PF, Giesy JP. 1983. Acute mortality of anthracene-
contaminated fish exposed to sunlight. Aquat. Toxicol. 3(1): 79-90.
14
40. Calfee RD, Little EE, Cleveland L, Barron MG. 1999. Photoenhanced Toxicity of a
Weathered Oil on Ceriodaphina dubia Reproduction. Environ. Sci. & Pollut. Res. 6(4):
208-212.
41. Cleveland L, Little EE, Calfee RD, Barron MG. 2000. Photoenhanced toxicity of
weathered oil to Mysidopsis bahia. Aquat. Toxicol. 49(1): 63-76.
42. Lyons BP, Pascoe CK, McFadzen IRB. 2002. Phototoxicity of pyrene and benzo(a)pyrene
to embryo-larval stages of pacific oyster Crassostrea gigas. Mar Environ Res, 54: 627–
631.
43. Holst LL, Giesy JP. 1989. Chronic effects of the photoenhanced toxicity of anthracene on
Daphnia magna reproduction. Environ Toxicol Chem. 8: 933-942.
44. Oris JT, Hall AT, Tylka JD. 1990. Humic Acids Reduce the Photo-induced Toxicity of
Anthracene to Fish and Daphina. Environ. Toxicol. 9: 575-583.
45. Oris JT, Giesy JP. 1986. Photoinduced toxicity of anthracene to juvenile bluegill sunfish
(Lepomis macrochirus Rafinesque): Photoperiod effects and predictive hazard
evaluation. Environ. Toxicol. Chem. 5: 761-768.
46. Peachy RBJ. 2005. The synergism between hydrocarbon pollutants and UV radiation: a
potential link between coastal pollution and larval mortality. J Ex Mar Biol Ecol. 315:
103-114.
47. Weinstein JE, Diamond SA. 2006. Relating Daily Solar Ultraviolet Radiation Dose in Salt
Marsh-associated Estuarine Systems to Laboratory Assessments of Photoactivated
Polycyclic Aromatic Hydrocarbon Toxicity. Environ. Toxicol. Chem. 25(11): 2860-2868.
48. Alloy MM, Boube I, Griffitt RJ, Oris JT, Roberts AP. 2015. Photo-induced Toxicity of
Deepwater Horizon Slick Oil to Blue Crab (Callinectes sapidus) Larvae. Environ. Toxicol.
Chem. 34(9): 2061-2066.
49. Alloy M, Baxter D, Stieglitz J, Mager E, Hoeing R, Benetti D, Grosell M, Oris J, Roberts A.
2015. Ultraviolet Radiation Enhances the Toxicity of Deepwater Horizon Oil to Mahi-
mahi (Coryphaena hippurus) Embryos. Environ Sci Technol. (in review).
50. Alloy M, Garner T, Bridges K, Mansfield C, Carney M, Forth H, Krasnec M, Lay C,
Takeshita R, Morris J, Bonnot S, Oris J, Roberts A. 2015. Sensitivity of early lifestage red
drum (Sciaenops ocellatus) and speckled seatrout (Cynoscion nebulosus) to photo-
induced toxicity of naturally weathered Deepwater Horizon oil. (In preparation).
51. Taylor L, et al. (In preparation).
52. Krylov SN, Huang X, Zeiler LF, Dixon DG, Greenberg BM. 1997. Mechanistic Quantitative
Structure-activity Relationship Model for the Photoinduced Toxicity of Polycyclic
Aromatic Hydrocarbons: I. Physical Model Based on Chemical Kinetics in a Two-
Compartment System. Enviro. Tox. Chem. 16(11): 2283-2295.
53. Hollis L, Burnison K, Playle RC. 1996. Does the age of metal-dissolved organic carbon
complexes influence binding of metals to fish gills? Aquat Toxicol. 35: 253-264.
15
54. Parkinson A, Roddick FA, Hobday MD. 2003. UV photooxidation of NOM: issues relating
to drinking water treatment. J Water Supply Res T. 52(8): 577-586.
55. Gilbert A, Baggott JE. 1991. Essentials of molecular photochemistry. CRC.
56. Wells CHJ. 1972. Introduction to Molecular Photochemistry. Chapman and Hall, London.
pp 1-13.
57. Estrada E, Patlewicz G. 2004. On the Usefulness of Graph-theoretic Descriptors in
Predicting Theoretical Parameters. Phototoxicity of Polycyclic Aromatic Hydrocarbons
(PAHs). Croat Chem ACTA. 77(1-2): 203-211.
58. Foote CS. 1991. Definition of type I and type II mechanisms of photosensitized oxidation.
Photochem. Photobiol. 54: 659.
59. Choi J, Oris JT. 2000. Evidence of oxidative stress in bluegill sunfish (Lepomis
macrochirus) liver microsomes simultaneously exposed to solar ultraviolet radiation and
anthracene. Environ. Toxicol. Chem. 19: 1795-1799.
60. Valenzeno DP. 1987. Photomodification and singlet oxygen generation in membranes.
In: Heitz JR Downum KR, Eds, Light-activated Pesticides. American Chemical Society,
Washington, DC. pp. 22-38.
61. Santamaria L, Giordano GG. 1969. Effects of long-wave ultraviolet radation on polycyclic
hydrocarbon carcinogenesis. In: Urbach MD, Ed., The Biological Effects of Ultraviolet
Radiation (with Emphasis on the Skin), Pergamon Press, New York. pp 569-580.
62. Weinstein JE, Oris JT, Taylor DH. 1997. An ultrastructural examination of the mode of
UV-induced toxic action of fluoranthene in the fathead minnow, Pimephales promelas.
Aquat Toxicol. 39: 1-22.
63. McCloskey JT, Oris JT. 1991. Effect of water temperature and dissolved oxygen
concentration on the photo-induced toxicity of anthracene to juvenile bluegill sunfish
(Lepomis macrohirus). Aquat Toxicol. 21: 145-156.
64. Caldecott KW. 2014. DNA single-strand break repair. Exp Cell Res. 329(1): 2-8.
65. Oris JT, Giesy JP. 1986. Photoinduced toxicity of anthracene to juvenile bluegill sunfish
(Lepomis macrochirus Rafinesque): Photoperiod effects and predictive hazard
evaluation. Environ. Toxicol. Chem. 5: 761-768.
66. Hatch AC, Burton Jr GA. 1999. Photo-induced toxicity of PAHs to Hyalella azteca and
Chironomus tentans: effects of mixtures and behavior. Environ pollut. 106(2): 157-167.
67. Seckmeyer G, Pissulla D, Glandorf M, Henriques D, Johnsen B, Webb A, Siani A, Bais A,
Kjeldstad B, Brogniez C, Lenoble J, Gardiner B, Kirsch P, Koskela T, Kaurola J, Uhlmann B,
Slaper H, den Outer P, Janouch M, Werle P, Grobner J, Mayer B, de la Casiniere A, Simic
S, Carvalho F. 2008. Variablity of UV Irradiance in Europe. Photochemistry and
Photobiology. 84: 172-179.
68. Madronich S, McKenzie RL, Björn LO, Caldwell MM. 1998. Changes in biologically active
ultraviolet radiation reaching the Earth’s surface. J Photoch Photobio B. 46: 5-19.
16
69. Lacis AA, Hansen JE. 1974. A Parameterization for the Absorption of Solar Radiation in
the Earth’s Atmosphere. J Atmos Sci. 31: 118-133.
70. Arts MT, Robarts RD, Kasai F, Waiser MJ, Tumber VP, Plante AJ, Rai H, de Lange, HJ.
2000. The Attenuation of Ultraviolet Radiation in High Dissolved Organic Carbon Waters
of Wetlands and Lakes on the Northern Great Plains. Limnol Oceanog. 45(2): 292-299.
71. Tedetti M, Sempere R. 2006. Penetration of Ultraviolet Radiation in the Marine
Environment: A Review. Photochem Photobiol. 82: 389-397.
72. Weinstein JE, Oris JT. 1999. Humic Acids Reduce the Bioaccumulation and Photoinduced
Toxicity of Fluoranthene to Fish. Environ Toxicol Chem. 18(9): 2087-2094.
73. Laurion I, Ventura M, Catalan J, Psenner R, Sommaruga R. 2000. Attenuation of
ultraviolet radiation in mountain lakes: factors controlling the among- and within-lake
variability. Limnol. Oceanogr. 45: 1274-1288.
74. Weinstein JE. 2003. Influence of Salinity on the Bioaccumulation and Photoinduced
Toxicity of Fluoranthene to an Estuarine Shrimp and Oligochaete. Environ. Toxicol.
Chem. 22(12): 2932-2939.
75. Ireland DS, Burton GA. Jr, Hess GG. 1996. In Situ Toxicity Evaluation of Turbidity and
Photoinduction of Polycyclic Aromatic Hydrocarbons. Environ. Toxicol. Chem. 15(4): 574-
581.
76. Little EE, Cleveland L, Clafee R, Barron MG. 2000. Assessment of the Photoenhanced
Toxicity of a Weathered Oil to the Tidewater Silverside. Environ. Toxicol. Chem. 19(4):
926-932.
77. Monson PD, Ankley GT, Kosian PA. 1995. Phototoxic response of Lumbriculus variegatus
to sediment contaminated by polycyclic aromatic hydrocarbons, short communication.
Environ. Toxicol. Chem. 14: 891-894.
78. Peachy RL, Crosby DG. 1995. Ultraviolet Radiation and Coral Reefs. UNIHI Sea Grant CR-
95-03. Phototoxicity in a coral reef flat community. HIMB Report #41: 193-200.
79. Maki H, Sasaki T, Harayama S. 2001. Photo-oxidation of biodegraded crude oil and
toxicity of the photo-oxidized products. Chemosphere. 44: 1145-1151.
80. Miller JS, Olejnik D. 2001. Photolysis of Polycyclic Aromatic Hydrocarbons in Water. Wat.
Res. 35(1): 233-243.
81. Nicodem DE, Guedes CLB, Fernandes CZ, Severino D, Correa RJ, Coutinho MC, Silva J.
2001. Photochemistry of Petroleum. Prog React Kinet Mec. 26: 219-238.
82. Wang Z, Fingas M, Blenkinsopp S, Sergy G, Landriault M, Sigouin L, Foght J, Semple K,
Westlake DWS. 1998. Comparison of oil composition changes due to biodegradation and
physical weathering in different oils. J Chromatogr A. 809: 89-107.
83. Duesterloh S, Short JW, Barron MG. 2002. Photoenhanced Toxicity of Weathered Alaska
North Slope Crude Oil to the Calanoid Copepods Calanus marshallae and Metridia
okhotensis. Environ. Sci. Technol. 36: 3953-3959.
17
84. McNutt MK, Camilli R, Crone TJ, Guthrie GD, Hsieh PA, Ryerson TB, Savas O, Shaffer F.
2012. Review of flow rate estimates of the Deepwater Horizon oil spill. Proc. Natl. Acad.
Sci. 109(50): 20260-20267.
85. Reddy CM, Arey JS, Seewald JS, Sylva SP, Lemkau KL, Nelson RK, Carmichael CA,
McIntyre CP, Fenwick J, Ventura GT, Van Mooy BAS, Camilli R. 2012. Composition and
fate of gas and oil released to the water column during the Deepwater Horizon oil spill.
PNAS. 109(50): 20229-20234.
86. Bejarano AC, Levine E, Mearns AJ. 2013. Effectiveness and potential ecological effects of
offshore surface dispersant use during the Deepwater Horizon oil spill: a retrospective
analysis of monitoring data. Environ. Monit. Assess. 185: 10281-10295.
87. Kujawinski EB, Soule MCK, Valentine DL, Boysen AK, Longnecker K, Redmond MC. 2011.
Fate of Dispersants Associated with the Deepwater Horizon Oil Spill. Environ. Sci.
Technol. 45: 1298-1306.
18
CHAPTER 2
PHOTO–INDUCED TOXICITY OF DEEPWATER HORIZON SLICK OIL TO BLUE CRAB (CALLINECTES
SAPIDUS) LARVAE1
Introduction
Polycyclic aromatic hydrocarbons (PAHs) are organic molecules with multiple carbon
ring structures that vary widely in their chemical and toxicological properties [1]. PAHs, as a
group, are lipophilic and readily accumulate in the tissues of aquatic organisms [2]. PAHs have
been shown to result in toxicity through a variety of mechanisms including photo-induced or
photo-enhanced toxicity [3,4]. Photo-induced toxicity is the phenomenon where a compound
exhibits increased toxicity in the presence of certain wavelengths of light [5]. Effects of PAH
photo-induced toxicity include increased mortality [6-10], reduced fecundity [3], increased
photo-avoidance behavior [11], and feeding inhibition [12]. The photo-induced toxicity of PAHs
to a wide variety of aquatic biota including daphnids [3, 13], fish [5, 6, 11, 14], bivalves [8],
marine corals [9], marine diatoms [15], and mysid shrimp [8, 10] is well documented.
Beginning on the 20th of April, 2010, the Mobile Offshore Drilling Unit Deepwater
Horizon (DWH) experienced a series of events that resulted in the sinking of the vessel and
subsequent oil release from the wellhead until it was sealed on July 15th, 2010. An estimated
700 million liters of oil was released, approximately 659 million liters more than the Exxon-
Valdez spill twenty-one years prior [16]. PAHs, including those with photodynamic activity, can
comprise a large fraction of crude oil [17].
1 This entire chapter is reproduced from Alloy, M. M., Boube, I., Griffitt, R. J., Oris, J. T., & Roberts, A. P. (2015).
Photo‐induced toxicity of Deepwater Horizon slick oil to blue crab (Callinectes sapidus) larvae. Environ. Toxicol. Chem., 34(9), 2061-2066, with permission from John Wiley and Sons.
19
The blue crab (Callinectes sapidus) ranges along the Western Atlantic coast as far north
as Nova Scotia, and as far south as Argentina [18]. It is found along the entire coastline of the
Gulf of Mexico and is a commercially and ecologically important species [18]. The mean yearly
blue crab hardshell harvest from the Gulf of Mexico from 2007 to 2011 was 75,846 metric tons,
and the mean blue crab softshell harvest for that time period was 847 metric tons [19]. In the
course of normal reproduction, blue crab release larva, known as zoea, into the water column
[20]. For the duration of their early life stages they remain in near-surface (<3 m) water where
they are likely to encounter UV light [20]. The goal of the current study was to determine the
sensitivity of blue crab zoea to photo-induced toxicity following exposure to DWH oil. To
accomplish this goal, zoea were exposed to a range of dilutions of DWH oil and gradations of
UV (natural sunlight filtered by plastics and mesh screening). Data from this study may be used
as a component of the Natural Resource Damage Assessment (NRDA) for blue crab following
the DWH oil spill.
Methods
Test organism
Organisms were obtained from two sources, the University of Southern Mississippi Gulf
Coast Research Lab (GCRL), and the University of Maryland Center for Environmental Science.
The source laboratories held their own adult brood stock and provided early lifestage Z3/Z4
zoea for testing. Prior to use in bioassays, zoea were held overnight (25 °C, 28-30 ppt salinity)
and fed rotifers obtained from the same in-house culture as the laboratory that provided the
zoea.
Test Solutions
20
Two field-collected oil samples were used in these experiments. Slick A is a surface slick
oil collected on July 29, 2010 from the hold of barge number CTC02404, which was receiving
surface slick oil from various skimmer vessels near the Macondo Well. Slick B is a more
weathered surface slick oil collected closer to shore on July 19, 2010 by the skimmer
vessel USCGC Juniper. Each of these oil samples are routinely used in testing as part of Natural
Resource Damage Assessment (NRDA). Synthetic seawater used as control/dilution water was
made by mixing BioSea Marine Mix (AquaCraft, Hayward, CA) with Milli-Q water to 28-30 ppt
salinity, 46 mS conductivity, and 8.0-8.4 pH.
Stocks of high energy water accommodated fraction (HEWAF) of Slick A or Slick B were
prepared by mixing a known volume of water with a mass of slick oil in a Waring C15 blender
(Stamford, Connecticut), on low power, for thirty seconds. The mixture was transferred to a
separatory funnel and allowed to settle in darkness for one hour before the lower portion was
drained for PAH analysis and utilization in test dilutions. Stocks of chemically enhanced water
accommodated fractions (CEWAF) using Slick A were prepared by known volume of water with
a mass of slick oil and dispersant (Corexit 9500) in a 10:1 ratio. The solution was stirred at a rate
sufficient to produce a vortex equal to 25% of solution height by a Teflon bar in a 4 L aspirator
bottle for at least 18 h prior to settling for one hour in darkness. The lower portion of the
solution was then drained for PAH analysis and utilization in test dilutions. Test dilutions were
prepared by dilution using synthetic seawater to a nominal percentage of HEWAF or CEWAF.
Samples of stocks and dilutions were taken with every preparation and shipped (4°C) to
ALS Environmental (Kelso, Washington) for analysis. PAH analytes were quantified using gas
chromatography mass spectroscopy in single ion monitoring mode (GC/MS-SIM), based on EPA
21
method 8270D [21]. The sum concentrations of 50 PAH analytes are reported and hereafter
referred to as tPAH50. Results of tPAH50 analyses for each test stock/renewal are reported in
Table 1.
Toxicity Tests
Zoea were exposed to a range of PAH concentrations and UV intensities in a factorial
design for 48 h. Exposures were conducted in 250 mL borosilicate glass crystallizing dishes
containing 10 zoea per dish. Two pairs of bioassays were conducted; (1) a Slick A HEWAF test
and a Slick A CEWAF test were conducted in parallel using Mississippi blue crab to examine
differences in toxicity related to WAF preparation, and (2) a Slick A HEWAF test and a Slick B
HEWAF test were conducted in parallel using Maryland blue crab (Mississippi crab were not
available) to examine differences in toxicity related to source oil. The exposure period for the
HEWAF/CEWAF pairing (Test 1) included an approximately 17 h equilibration period (i.e.,
exposure to WAF in darkness) followed by a morning WAF renewal, a 7 h solar exposure, an
overnight recovery period (17 h) followed by a second WAF renewal, a second 7 h solar
exposure, and an overnight recovery period (17 h). At the end of this 48h total exposure
period, mortality was assessed. The exposure regime for the Slick A/B HEWAF pairing (Test 2)
was similar, except that test media was renewed only once (at the end of the first solar
exposure) and mortality was assessed immediately after the second solar exposure, forgoing
the second overnight recovery period. Each bioassay had five PAH treatments with three to five
replicate dishes per PAH treatment. Tests conducted with Mississippi blue crab were carried
out using two UV treatments (10% and 100% ambient sunlight). Tests conducted with Maryland
blue crab were conducted using three UV treatments (10%, 50%, and 100% ambient sunlight).
22
Replicate dishes were suspended in an outdoor, flow-through water bath to maintain
temperature. Dishes were floated in polystyrene foam insulation board with holes cut to hold
replicate dishes in contact with the temperature bath water across the underside, and the
majority of the sidewall. Sunlight was used as the source of UV radiation. Screening materials
OP-4 (Professional Plastics, Fullerton, CA) plastic sheet transparent to UV (>90%) was used for a
full intensity (100% ambient) UV treatment. A metal mesh screen was added over the top of the
OP-4 plastic as an additional filter to achieve an approximately 50% ambient UV treatment. A
different formulation of acrylic, OP-3 (Professional Plastics, Fullerton, CA), plastic sheet allowed
transmittance of less than 10% of ambient UV. UV was measured continuously during the
exposures using a Biospherical PUV2500 radiometer (BioSpherical Instruments, San Diego, CA).
For each bioassay, organisms were loaded into dishes containing one of five test
dilutions and allowed to acclimate overnight in the absence of UV. After this period, dishes
were placed in the outdoor testing apparatus and exposed to approximately 7 h of sunlight,
referred to hereafter as the first solar exposure. At the end of 7 hours, dishes were taken to
shaded shelter where test solutions were renewed and survival recorded. Replicates remained
in the shelter for an overnight dark period. The following morning, test replicates were taken to
the outdoor testing apparatus for a second solar exposure. Survival was again assessed after
this second solar exposure.
Phototoxic Units
All tests were performed outdoors using ambient UV. Tests not performed in parallel
received different UV doses as a result. To account for differences in UV co-exposure, a
23
phototoxic unit was calculated using methods similar to Oris and Giesy [5]. Fourteen known
phototoxic PAHs present in the WAF preparations were used in the calculations: anthracene,
benzo[a]anthracene, benzo[e]pyrene, benzo[g,h,i]perylene, chrysene, fluoranthene, fluorene
(as well as C1 and 2), phenanthrene (as well as C1, 2, and 3), and pyrene. The aqueous
concentration of each PAH was calculated as a molar value and multiplied by its relative
photodynamic activity (RPA) compared to anthracene. The sum of each PAH’s molar
concentration multiplied by its RPA was used to calculate the sum equivalent molar
concentration of anthrancene. UV irradiances are reported as the integration of the test
duration at a resolution of one second, expressed as mW∙s/cm2. The anthracene equivalent
concentration is multiplied by the integration of the UV irradiance at λ=380nm.
Phototoxic dose =
Where ‘mW∙s’ only refers to the integration of irradiance at λ=380nm. Phototoxic units
are expressed as µM/L∙mW∙s/cm2.
Statistical Analyses
For each bioassay, a 2-factor analysis of variance (ANOVA) with a Dunnet’s post-hoc test
was used to determine differences in survival (percent survival data was arcsine-transformed to
meet ANOVA assumptions) between treatments in the statistical software JMP (version 11 SAS
Institute, Cary, NC). In each of the four ANOVAs, the factors were UV treatment, and tPAH50
concentration. Median lethal concentrations (LC50) were calculated using the drc package [22]
% WAF Initial tPAH50 1st Renewal 2nd Renewal
24
(µg/L) tPAH50 (µg/L) tPAH50 (µg/L)
Slick A HEWAF
Mississippi zoea 0% 0.03 0.45 0.16
0.08% 1.90 1.32 1.03
0.4% 8.42 6.02 4.58
2% 44.02 16.40 18.20
10% 208.95 88.48 68.75
Slick A CEWAF
Mississippi zoea 0% 0.03 0.45 0.16
1% 2.46 1.08 0.40
5% 3.74 4.71 1.94
15% 72.23 16.82 5.58
20% 76.54 28.61 8.37
Slick A HEWAF Maryland
zoea 0% 0.02 0.01 --
0.75% 14.71 13.56 --
1.50% 28.34 28.88 --
3% 54.09 58.17 --
6% 127.91 115.64 --
Slick B HEWAF Maryland
zoea 0% 0.02 0.02 --
3.50% 9.65 10.00 --
7.50% 19.03 16.11 --
15% 37.98 34.93 --
30% 71.81 66.89 --
Table 1. The nominal test dilution in percent of stock WAF (1g/L oil) and the measured tPAH50 concentration of the initial exposure and renewal solutions. “–“ indicates that there was no second renewal.
Results
Toxicity Associated with WAF Preparation
Parallel tests with Mississippi blue crab were designed to examine toxicity associated
with differences in WAF preparation (HEWAF vs CEWAF). In both the HEWAF and CEWAF
assays, organisms were exposed to two gradations of UV (100% and 10% ambient sunlight).
Organisms in the 100% ambient UV treatment were exposed to a mean intensity (± 1 SD) of
0.035 ± 0.024 mW/cm2/s and a cumulative, integrated dose of 908.2 mW·s/cm2 for the first
25
solar exposure and a mean intensity of 0.051 ± 0.026 mW/cm2/s and a cumulative dose of
1570.3 mW·s/cm2 for the second solar exposure. Organisms in the 10% ambient UV treatment
were exposed to a mean intensity of 0.004 ± 0.002 mW/cm2/s and a cumulative, integrated
dose of 90.8 mW·s/cm2 for the first solar exposure and a mean intensity of 0.005 ± 0.003
mW/cm2/s and a cumulative dose of 157 mW·s/cm2 for the second solar exposure. Both assays
also consisted of five PAH exposure concentrations. Measured tPAH50 concentrations in the
HEWAF exposure solutions were 0.03, 1.90, 8.42, 44.02, and 208.95 µg/L. Measured tPAH50
concentrations in CEWAF exposure solutions were 0.03, 2.46, 3.74, 72.23, and 76.54 µg/L.
In the HEWAF test, 100% ambient UV treatment, there were significant decreases in
survival at 44.02 µg /L compared to controls including 100% mortality in the 208.95 µg/L tPAH50
treatment (p<0.01) (Figure 1A). The phototoxic dose LC50 was 20.6 µM/L·mW∙s/cm2 (9.7-31.5
µM/L·mW∙s/cm2) in the HEWAF test. There were no significant differences in survival among
any PAH or UV treatment in the CEWAF test (p=0.07) (Figure 1B). There was insufficient
mortality to calculate a phototoxic LC50 from the CEWAF test.
Toxicity Associated with Oil Source
Parallel tests with Maryland blue crab were designed to examine differences associated
with oil samples (i.e. Slick A vs. Slick B). Because no toxicity was observed in CEWAF
preparations at the tPAH50 concentrations tested, these assays were run only with HEWAF
preparations. In both toxicity assays, organisms were exposed to one of three gradations of UV
(10%, 50%, and 100% ambient sunlight). Organisms in the 100% ambient UV treatment were
exposed to a mean intensity of 0.076 ± 0.009 mW/cm2/s and a cumulative, integrated dose of
1904.4 mW·s/cm2 for the first solar exposure, and a mean intensity of 0.044 ± 0.028 mW/cm2/s
26
and a cumulative dose of 1058 mW·s/cm2 for the second solar exposure. Organisms in the 50%
ambient UV treatment were exposed to a mean intensity of 0.038 ± 0.005 mW/cm2/s and a
cumulative, integrated dose of 952.2 mW·s/cm2 for the first solar exposure, and a mean
intensity of 0.022 ± 0.014 mW/cm2/s and a cumulative dose of 529 mW·s/cm2 for the second
solar exposure. Organisms in the 10% ambient UV treatment were exposed to a mean intensity
of 0.008 ± 0.001 mW/cm2/s and a cumulative, integrated dose of 190.4 mW·s/cm2 for the first
solar exposure, and a mean intensity of 0.004 ± 0.003 mW/cm2/s and a cumulative dose of
105.8 mW·s/cm2 for the second solar exposure. Both assays also consisted of five PAH exposure
concentrations. Measured Slick A tPAH50 concentrations in the exposure solutions were 0.02,
14.71, 28.34, 54.09, and 127.91 µg/L. Measured Slick B tPAH50 concentrations were 0.02, 9.65,
19.03, 37.98, and 71.81 µg/L.
In the Slick A test, survival was reduced by 74%, relative to controls, in the 127.91 µg/L
tPAH50 concentration in the 10% ambient UV treatment relative to controls (p=0.02). In the 50%
ambient UV treatment, significant decreases in survival were observed at tPAH50
concentrations ≥28.34 µg/L resulting in less than 10% survival (p<0.01). In the 100% ambient
UV treatment, significant decreases in survival (<20% survival) were observed in all tested
tPAH50 concentrations except the 0.02 µg/L controls (p<0.01) (Figure 2A). The phototoxic dose
LC50 was 9.5 µM/L·mW∙s/cm2 (8.1-10.8 µM/L·mW∙s/cm2) in the Slick A test.
In the Slick B test, there was no significant reduction in survival relative to controls in
the 10% ambient UV treatment. In the 50% ambient UV treatment, survival at tPAH50
concentrations ≥19.03 µg/L was less than 10%, and significantly reduced compared to control
survival (p<0.01). In the 100% ambient UV treatment, survival was significantly reduced to less
27
than 10% at all tPAH50 concentrations except the 0.02 µg/L controls (p<0.01) (Figure 2B). The
phototoxic dose LC50 was 9.9 µM/L·mW∙s/cm2 (9.4-10.5 µM/L·mW∙s/cm2) in the Slick B test.
28
Figure 1. Mean percent survival (± 1 SE) in Mississippi blue crab zoea exposed to [A] Slick A HEWAF or [B] Slick A CEWAF after two 7-h solar exposures. Asterisks indicate treatments with mean percent survival significantly different from controls within that UV treatment. Percent survival of each replicate by the log10 phototoxic dose + 1 of Mississippi blue crab zoea exposed to [C] Slick A HEWAF or [D] Slick A CEWAF.
29
Figure 2. [A] Mean percent survival (± 1 SE) of Maryland zoea exposed to [A] Slick A HEWAF or [B] Slick B HEWAF after two 7 h solar exposures. Asterisks mark treatments with mean percent survival significantly different from controls within that UV treatment. Percent survival of each replicate by the log10 phototoxic dose + 1 of Mayland blue crab zoea exposed to [C] Slick A HEWAF or [D] Slick B HEWAF.
30
Discussion
Standard laboratory-based toxicity testing underestimates acute PAH toxicity by not
accounting for interactions with natural stressors such as UV. In general, this study
demonstrates that low UV exposures required ten-fold more PAH compound to induce median
mortality compared to high UV exposures. The values generated in this study are comparable to
those reported by other investigators in studies of PAH photo-induced toxicity in marine
invertebrates [23, 24]. Concentrations of PAH which elicited significant acute mortality in the
presence of UV (0.3-12.9 µg/L) fall within the range of PAH concentrations reported in surface
waters during the Deepwater Horizon oil spill (0-84.8 µg/L) [25]. Furthermore, the measured
tPAH50 values are based on samples taken immediately after WAF preparation and do not
account for loss of PAH over time in the exposure chambers before renewal. Thus, the toxicity
values reported here are conservative and may underestimate toxicity. This demonstrates that
a UV component should be included in studies assessing the toxicity of PAHs to aquatic
organisms that may be exposed to UV in their habitats or injury to these organisms may be
greatly underestimated.
WAF preparation method had a significant effect on the occurrence of photo-induced
toxicity in blue crab larvae. The measured tPAH50 concentrations in the higher dilutions of
CEWAF fall within the range of values observed to result in significant toxicity in HEWAF
preparations. However, no significant toxicity, photo-induced or otherwise, was observed in
CEWAF preparations. This implies that the use of dispersants could reduce phototoxic hazard to
blue crab zoea. Previous investigations into dispersed oil toxicity have reported combinations of
oil and dispersant to be as toxic as oil alone [26], to reduce toxicity compared to oil-only
31
exposures [27], or to exhibit enhanced toxicity [28], as well as greater potential for
bioaccumulation [29, 30]. These previous investigations did not examine photo-induced
toxicity, and many of the test concentrations were tenfold higher or more than what was
utilized in the present study’s CEWAF assay. The highest Corexit exposure and its PAH
concentration are well below the reported NOECs in the studies cited above. This would imply
that while the addition of dispersant mediates photo-induced toxicity, the exposures in the
present study were below the threshold for non-UV acute toxicity.
The mechanism by which dispersant mediates photo-induced toxicity is unknown. Some
published models of photo-induced toxicity use PAH body burden as a predictor variable and
not waterborne PAH concentration [31]. Body burdens of PAH in larval blue crab were not
determined largely due to logistics and size and availability limitations of the test organisms.
However, a recent investigation has reported that in small bodied organisms (i.e. embryos or
larva with high surface area to body volume ratios), tissue concentrations did not significantly
improve model accuracy over water borne concentrations [31]. It is possible that dispersant
alters the bioavailability of PAH, reducing the rate of uptake [29]. Previous studies have
suggested it could increase bioaccumulation [30]. HEWAF preparations may contain more
bioavailable PAH through an as yet undetermined mechanism. It is also possible that dispersant
may absorb specific wavelengths of UV radiation, thus reducing the number of photochemical
reactions at the tissue level. Or, dispersion may enhance photolysis and loss of PAH over time in
the exposure systems. Further investigation into the mechanism by which dispersants mediate
photo-induced toxicity is warranted as dispersants were widely utilized in the Deepwater
Horizon incident, as well as many other accidental oil releases.
32
In addition to the concentration of phototoxic PAHs, toxicity assessments will need to
consider the intensity of UV radiation and its penetration in marine surface waters. In the
present study, UV radiation intensity was varied to artificially simulate surface radiation with
minimal attenuation as well as depths where UV intensity is reduced to half, and to one tenth
of surface intensities. UV radiation attenuates with depth, and the rate of attenuation is
dependent on a variety of factors (dissolved organic carbon, suspended particulates, plankton
density, etc.) that vary on a site by site basis [32]. In open water areas of the Gulf of Mexico,
UV-A Z10 (the depth at which only 10% of surface UV-A irradiance remains) can be as deep as 37
m [32]. In coastal areas, UV attenuation varies greatly, and Z10 values as deep as 5 m and as
shallow as <1 m have been reported [32]. The high rates of UV attenuation in coastal waters are
primarily caused by non-photobleached dissolved organic carbon influx and suspended
particulates from freshwater inputs [33]. However, these are subject to great stochastic
variation. In order to extrapolate the results of the toxicity tests presented here to
invertebrates in the field, assessments of field UV exposure should be considered.
We have shown that co-exposure to slick oil from the Deepwater Horizon spill and
sunlight results in photo-induced toxicity in blue crab larvae. Effects were observed well within
the range of tPAH50 concentrations reported during the spill [25] and during relatively short
exposure periods (<48 h). Toxicity was most prevalent in HEWAF oil preparations, with no
toxicity observed in CEWAF preparations at the concentrations tested. The data from this study
combined with literature reports on UV penetration in the Gulf of Mexico demonstrate that
photo-induced toxicity of PAH should be considered in natural resource damage assessments of
the Deepwater Horizon oil spill. However, predicting actual PAH exposure and UV intensities
33
experienced by blue crab zoea in the Gulf of Mexico during the spill is outside the scope of this
study. The toxicity data presented here should be an important consideration for potential
effects of the Deepwater Horizon oil spill and future oil spills.
Acknowledgements
Data presented here are a subset of a larger toxicological database that is being
generated as part of the Deepwater Horizon Natural Resource Damage Assessment, therefore,
these data will be subject to additional analysis and interpretation which may include
interpretation in the context of additional data not presented here.
This work was supported as part of the Deepwater Horizon Natural Resource Damage
Assessment (NRDA). Data presented here are a subset of a larger toxicological database that is
being generated as part of the Deepwater Horizon NRDA, therefore, these data will be subject
to additional analysis and interpretation which may include interpretation in the context of
additional data not presented in this publication. The authors thank Stratus Consulting,
particularly Jeff Morris, Heather Forth, and Claire Lay, for their contributions. Thanks to
University of Southern Mississippi Gulf Coast Research Lab, and the University of Maryland for
providing test organisms.
34
References
1. Douben, Peter ET. 2003. Assessing Risks from Photoactivated Toxicity of PAHs to
Aquatic Organisms. In PAHs: An Ecological Perspective; Gerald T. Ankley, Lawrence P.
Burkhard, Philip M. Cook, Stephen A. Diamond, Russell J. Erickson and David R.
Mount. John Wiley & Sons Ltd. West Sussex, England. pp 273-296.
2. Baumard P, Budzinski H, Garrigues P, Sorbe JC, Burgeot T, Bellocq J. 1998.
Concentrations of PAHs (polycyclic aromatic hydrocarbons) in various marine
organisms in relation to those in sediments and to trophic level. Marine Pollution
Bulletin, 36(12): 951-960.
3. Holst LL, Giesy JP. 1989. Chronic effects of the photoenhanced toxicity of anthracene
on Daphnia magna reproduction. Environmental Toxicology and Chemistry, 8(10):
933-942.
4. Diamond SA, Milroy NJ, Mattson VR, Heinis LJ, Mount DR. 2003. Photoactivated
toxicity in amphipods collected from polycyclic aromatic hydrocarbon–contaminated
sites. Environmental toxicology and chemistry, 22(11): 2752-2760.
5. Oris JT, Giesy JP. 1987. The photo-induced toxicity of polycyclic aromatic
hydrocarbons to larvae of the fathead minnow (Pimephales promelas).
Chemosphere, 16(7): 1395-1404.
6. Bowling JW., Leversee GJ, Landrum PF, Giesy JP. 1983. Acute mortality of
anthracene-contaminated fish exposed to sunlight. Aquatic Toxicology, 3(1): 79-90.
7. Boese BL, Lamberson JO, Swartz RC, Ozretich RJ. 1997. Photoinduced toxicity of
fluoranthene to seven marine benthic crustaceans. Archives of environmental
contamination and toxicology, 32(4): 389-393.
8. Pelletier MC, Burgess RM, Ho KT, Kuhn A, McKinney RA, Ryba SA. 1997. Phototoxicity
of individual polycyclic aromatic hydrocarbons and petroleum to marine
invertebrate larvae and juveniles. Environmental toxicology and chemistry, 16(10):
2190-2199.
9. Peachey RL, Crosby DG. 1995. Phototoxicity in a coral reef flat community. UV
Radiation and Coral Reefs, HIMB Tech. Report, 41:193-200.
10. Cleveland L, Little EE, Calfee RD, Barron MG. 2000. Photoenhanced toxicity of
weathered oil to Mysidopsis bahia. Aquatic toxicology, 49(1): 63-76.
11. Oris JT, Giesy JP. 1986. Photoinduced toxicity of anthracene to juvenile bluegill
sunfish (Lepomis macrochirus Rafinesque): Photoperiod effects and predictive
hazard evaluation. Environmental toxicology and chemistry, 5(8): 761-768.
12. Hatch AC, Burton GA. 1999. Photo-induced toxicity of PAHs to Hyalella azteca and
Chironomus tentans: effects of mixtures and behavior. Environmental
pollution, 106(2): 157-167.
35
13. Allred PM, Giesy JP. 1985. Solar radiation‐induced toxicity of anthracene to Daphnia
pulex. Environmental Toxicology and Chemistry, 4(2): 219-226.
14. Diamond SA, Mount DR, Mattson VR, Heinis LJ, Highland TL, Adams AD, Simcik MF.
2006. Photoactivated polycyclic aromatic hydrocarbon toxicity in medaka (Oryzias
latipes) embryos: relevance to environmental risk in contaminated
sites. Environmental toxicology and chemistry, 25(11): 3015-3023.
15. Wang L, Zheng B, Meng W. 2008. Photo-induced toxicity of four polycyclic aromatic
hydrocarbons, singly and in combination, to the marine diatom Phaeodactylum
tricornutum. Ecotoxicology and environmental safety, 71(2): 465-472.
16. McNutt MK, Camilli R, Crone TJ, Guthrie GD, Hsieh PA, Ryerson TB, Savas O, Shaffer
F. 2012. Review of flow rate estimates of the Deepwater Horizon oil
spill. Proceedings of the National Academy of Sciences, 109(50): 20260-20267.
17. Atlas RM. 1975. Effects of temperature and crude oil composition on petroleum
biodegradation. Applied Microbiology, 30(3): 396-403.
18. Synopsis of Biological Data on the Blue Crab, Callinectes sapidus (Rathbun); NOAA
Technical Report NMFS-1, 1984
19. NOAA. 2014. US Commercial Landings 2011-2012; National Marine Fisheries Service.
Available from:
https://www.st.nmfs.noaa.gov/Assets/commercial/fus/fus12/02_commercial2012.p
df
20. Epifanio CE. 1995. Transport of blue crab (Callinectes sapidus) larvae in the waters
off mid-Atlantic states. Bulletin of Marine Science, 57(3): 713-725.
21. SW-846 Manual for Waste Testing; United States Environmental
Protection Agency: Washington, DC, 1986; Vols. 1B and 1C.
22. Ritz C, Streibig JC. 2005. Bioassay Analysis using R. Journal of Statistical Software.
12(5).
23. Fathallah S, Medhioub MN, Kraiem MM. 2012. Photo-induced Toxicity of Four
Polycyclic Aromatic Hydrocarbons (PAHs) to Embryos and Larvae of the Carpet Shell
Clam Ruditapes decussatus. Bulletin of environmental contamination and
toxicology, 88(6): 1001-1008.
24. Peachy RBJ, 2005. The synergism between hydrocarbon pollutants and UV radiation:
a potential link between coastal pollution and larval mortality. Journal of
Experimental Marine Biology and Ecology, 315: 103-114.
25. Diercks AR, Highsmith RC, Asper VL, Joung D, Zhou Z, Guo L, Shiller AM, Joye SB,
Teske AP, Guinasso N, Wade TL, Lohrenz SE. 2010. Characterization of subsurface
polycyclic aromatic hydrocarbons at the Deepwater Horizon site. Geophysical
Research Letters, 37: L20602
36
26. Adams J, Sweezey M, Hodson PV, 2014. Oil and oil disperstant does not cause
synergistic toxicity to fish embryos. Environmental Toxicology and Chemistry, 33 (1):
107-114.
27. Fuller C, Bonner J, Page C, Ernest A, McDonald T, McDonald S. 2004. Comparative
toxicity of oil, dispersant, and oil plus dispersant to several marine species.
Environmental Toxicology and Chemistry, 23 (12): 2941-2949.
28. Kuhl AJ, Nyman JA, Kaller MD, Green CC. 2013. Dispersant and salinity effects on
weathering and acute toxicity of South Louisiana Crude oil. Environmental
Toxicology and Chemistry, 32 (11): 2611-2620.
29. Van Scoy AR, Voorhees J, Anderson BS, Philips BM, Tjeerdema RS. 2013. Use of
semipermeable membrane devices (SPMDs) to characterize dissolved hydrocarbon
fractions of both dispersed and undispersed oil. Environmental Science Processes &
Impacts, 15: 2016-2022.
30. Ramachandran SD, Hodson PV, Kahn CW, Lee K. 2004. Oil dispersant increases PAH
uptake by fish exposed to crude oil. Ecotoxicology and Environmental Safety, 59:
300-308.
31. Willis AM, Oris JT. 2014. Acute photo-induced toxicity and toxicokinetics of single
compounds and mixtures of polycyclic aromatic hydrocarbons in zebrafish.
Environmental Toxicology & Chemistry, 33(9): 2028-2037.
32. Tedetti M, Sempere R. 2006. Penetration of Ultraviolet Radiation in the Marine
Environment. A Review. Photochemistry and Photobiology, 82: 389-397.
33. Shank GC, Evans A. 2011. Distribution and photoreactivity of chromophoric dissolved
organic matter in northern Gulf of Mexico shelf waters. Continental Shelf Research,
31: 1128-1139.
37
CHAPTER 3
ULTRAVIOLET RADIATION ENHANCES THE TOXICITY OF DEEPWATER HORIZON OIL TO MAHI-
MAHI (CORYPHAENA HIPPURUS) EMBRYOS
Introduction
Polycyclic aromatic hydrocarbons (PAHs) are a class of organic molecules composed of
multiple benzene rings that vary widely in their chemical and toxicological properties [1]. As a
group, PAHs are lipophilic and readily bioaccumulate [2]. PAHs exert toxicity through several
mechanisms including photo-induced toxicity [3-5]. Photo-induced toxicity is a phenomenon in
which a compound exhibits increased toxicity in the presence of certain wavelengths of light
[6]. Photodynamic PAHs, including those found in crude oil [7], have been shown to result in
photo-induced toxicity in aquatic organisms [5, 8-10]. Effects of PAH photo-induced toxicity
include increased mortality [1, 8, 11-14], reduced fecundity [3], increased photo-avoidance
behavior [15], and feeding inhibition [16].
Beginning on the 20th of April, 2010, the Mobile Offshore Drilling Unit Deepwater
Horizon experienced a series of events that resulted in the sinking of the vessel and subsequent
release of oil from the wellhead until it was sealed on July 15th, 2010 [17]. We have previously
shown that oil from the Deepwater Horizon spill is phototoxic to early lifestage blue crab at PAH
concentrations within the range of those that occurred during the spill [10]. The timespan and
scale of the oil release presented a hazard to both near-shore species such as the blue crab and
open water species like the mahi-mahi. While photo-induced toxicity of PAHs to fishes has been
reported [5, 11, 15, 18-20], little is known with respect to commercially and ecologically
38
relevant pelagic fish species that likely resided in the Gulf of Mexico at the time of the spill [21,
22].
The mahi-mahi (Coryphaena hippurus) occurs in almost every ocean body lower than 30
degrees in latitude with local distributions sometimes ranging farther north and south with
warmer currents [23]. It is found throughout the Gulf of Mexico and is an important
recreational resource as well as a commercially fished species [24]. The mean combined annual
mahi-mahi commercial and recreational harvest from the Gulf of Mexico from 2000 to 2012
was 980 metric tons [24]. In the course of a single reproductive event, mahi-mahi females
release as many as 1.5 million buoyant embryos in offshore waters [25]. For the duration of
their embryonic life stage the eggs remain buoyant in surface water where they are likely to
encounter UV light [25]. Due to the relative transparency, and positive buoyancy of their
embryos during early development, we hypothesized that mahi-mahi embryos would
specifically be at risk to photo-induced toxicity following exposure to PAHs. To test this
hypothesis, mahi-mahi embryos were exposed to a range of dilutions of water accommodated
fractions (WAF) of artificially weathered source oil, or to slick oil. Exposures were carried out
under gradations of UV achieved using natural sunlight filtered by plastics and mesh screening.
Data from this study may be used as a component of the Natural Resource Damage Assessment
(NRDA) following the DWH oil spill.
Materials and Methods Test organism
Organisms were obtained from a wild cohort of mahi-mahi broodstock maintained at
the University of Miami. Spawning occurred at dawn and embryos were collected in a purpose-
39
built egg collection vessel that was attached to a recirculating broodstock maturation system.
Embryos were prepared using methods described in Stieglitz et al., 2012 [26], whereby viable
embryos were treated with a formalin solution to remove parasites prior to use in toxicological
tests.
Test Solutions
Two source oils were used in these experiments, a field collected oil and an artificially
weathered oil. The field oil was obtained on July 29, 2010 from the hold of barge number
CTC02404, which was receiving surface slick oil from various skimmer vessels near the
Macondo Well. This slick oil is routinely used in NRDA testing for the Deepwater Horizon spill.
The artificially weathered oil was obtained from the MC252 riser. Artificial weathering was
accomplished using methods modified from Carls et al [24]. Oil was heated to approximately
98°C and stirred lightly until its mass was reduced by 33 to 38 percent. Filtered, UV-sterilized
Atlantic seawater was used in control/dilution preparations. Water physico-chemical
parameters were within the following ranges, 30-34 ppt salinity, 49-55 mS conductivity, and
7.9-8.4 pH.
Stocks of high energy water accommodated fraction (HEWAF) were prepared prior to
each test by mixing a known volume of water with a mass of slick oil in a Waring CB15 blender
(Stamford, Connecticut), on low power, for thirty seconds. The mixture was transferred to a
separatory funnel and allowed to settle in darkness for one hour before sampling for PAH
analysis and utilization in test dilutions. Stocks of chemically enhanced water accommodated
fractions (CEWAF) using were prepared by known volume of water with a mass of slick oil and
dispersant (Corexit 9500) in a 10:1 ratio. In darkness, the solution was stirred by a Teflon bar at
40
sufficient speed to achieve a 25% vortex in a 2 L aspirator bottle for 18-24 h prior to settling for
one hour. The solution was then sampled for PAH analysis and utilization in test dilutions. Test
dilutions were prepared by serial dilution in synthetic seawater to a nominal percentage of
HEWAF or CEWAF. All stocks were made to the same mass ratio of oil to water.
Samples of stocks and dilutions were taken with every preparation and shipped (4°C) to
Analytical Laboratory Services (Kelso, Washington) for analysis. Fifty specific PAH analytes were
quantified using gas chromatography mass spectroscopy in single ion monitoring mode
(GC/MS-SIM), based on EPA method 8270D [28]. The sum concentrations of these 50 PAH
analytes are hereafter referred to as tPAH50.
Toxicity Tests
The investigation consisted of four separate toxicity tests in which mahi-mahi embryos
were exposed to either CEWAF derived from slick oil, CEWAF derived from artificially
weathered source oil, HEWAF derived from slick oil, or HEWAF derived from artificially
weathered source oil. This approach allowed the investigation into the possible differences in
photo-induced toxicity brought about by dispersant based WAF preparation versus mechanical
WAF preparation, and possible differences from slick oil or artificially weathered oil used in
WAF preparations.
Mahi-mahi embryos were exposed to one of a range of PAH concentrations combined
with two or three UV intensities in a factorial design for 48 h. Exposures were conducted in 250
mL borosilicate glass crystallizing dishes containing 10 embryos per dish. The exposure period
included an approximately 17 h equilibration period, a 7 h solar exposure, an overnight
recovery period (17 h), a second 7 h solar exposure, and an overnight recovery period after
41
which percent hatch in each replicate was assessed. Each toxicity test had five to six PAH
treatments with five replicate dishes per PAH treatment.
Replicate dishes were suspended in an outdoor, flow-through water bath to maintain
temperature. Dishes were floated in polystyrene foam insulation board with holes cut to hold
replicate dishes in contact with the temperature bath water across the underside, and the
majority of the sidewall. Sunlight was used as the source of UV radiation. Screening materials
were suspended over replicate dishes to achieve gradations of UV (λ = 380 nm). A specially
formulated plastic sheet >90% transparent to UV was used for a full intensity (100% ambient)
UV treatment (KNF Corporation, Tamaqua, Pennsylvania, USA). A metal mesh screen was added
over the top of the full intensity plastic as an additional filter to achieve an approximately 50%
ambient UV treatment. A different formulation of plastic sheet allowing transmission of <10%
of ambient UV (Rosco Laboratories Inc, Stamford, Connecticut, USA) was used as a control. UV
was measured continuously during the exposures using a Biospherical radiometer (BioSpherical
Instruments, San Diego, CA).
Phototoxic Units
All tests were performed outdoors using ambient sunlight as a source of UV. Tests
performed on different days received different UV doses. To account for differences in UV co-
exposure, a phototoxic unit was calculated as described previously in Alloy et al. [10] using
methods similar to Newsted and Giesy [6]. Concentrations of fourteen known phototoxic PAHs
were used in the calculations: anthracene, benzo[a]anthracene, benzo[e]pyrene,
benzo[g,h,i]perylene, chrysene, fluoranthene, fluorene (as well as C1 and 2), phenanthrene (as
well as C1, 2, and 3), and pyrene. The aqueous concentration of each PAH was calculated as a
42
molar value and multiplied by its relative photodynamic activity compared to anthracene (RPA).
This produced the sum equivalent molar concentration of anthracene. This anthracene
equivalent concentration was multiplied by the integration of the UV irradiance (λ=380nm) to
produce the phototoxic dose. UV irradiances are reported as the integration of the test
duration at a resolution of one second, expressed as mW∙s/cm2. Phototoxic units are expressed
as µM/L·mW∙s/cm2.
Statistical Analyses
For each toxicity test, hatch data was arcsine transformed and a 2-factor analysis of
variance (ANOVA) with a Dunnett’s post-hoc test was used to determine differences in percent
hatch using the statistical software JMP (version 11, SAS Institute, Cary, NC). All statistical
comparisons were made using α= 0.05. UV treatment and tPAH50 concentration were used as
factors in each ANOVA. Median effect concentrations (EC50) for phototoxic dose were
calculated using the drc package in R (version 3.1.2) [29].
A table was generated of the anthracene equivalent molar concentrations required at a
given UV dose to meet three effect concentrations was generated using the mean UV intensity
of all tests, and the calculated effect concentrations for twenty percent, fifty percent, and
eighty percent. The mean UV intensity was multiplied by an exposure duration of 16 hours. This
UV dose was used as the 100% UV exposure for the table, and was reduced accordingly for
75%, 50%, and 25% UV calculations.
Results
Slick oil CEWAF dilutions contained 0.4, 1.5, 2.7, 5.1, and 10.0 µg/L tPAH50. The total UV
dose in each exposure was calculated by integrating the total irradiance received over the
43
timecourse of the test during both solar exposure periods. The slick oil CEWAF test utilized
three gradations of UV (100%, 50%, and 10%). Slick oil CEWAF 100% UV exposures received a
total integrated dose of 3276 mW·s/cm2 with a mean intensity (+/- 1SD) of 0.053 ± 0.023
mW/cm2/s. Significant toxicity was observed at exposures ≥ 2.7 µg/L tPAH50 in the 100% UV
treatment only (p < 0.001) (Figure 1A). To account for differences in UV exposure between
tests, EC50s were calculated in phototoxic dose units for each test. The slick oil CEWAF
phototoxic EC50 was 11.8 µM/L·mW∙s/cm2 (95% confidence interval = 7.84-15.7
µM/L·mW∙s/cm2) (Figure 1B).
Slick oil HEWAF dilutions contained 0, 0.1, 0.3, 0.9, 4.3, and 20.9 µg/L tPAH50. The slick
oil HEWAF test utilized two gradations of UV (100% and 10%) only. Slick oil HEWAF 100% UV
exposures received an integrated dose of 3022 mW·s/cm2 with a mean intensity of 0.044 ±
0.022 mW/cm2/s. Significant toxicity was observed to occur at exposures ≥ 5.0 µg/L tPAH50 in
the 100% UV treatment, and at the 20.9 µg/L tPAH50 exposures in the 10% UV treatment (p <
0.001) (Figure 1C). The slick oil HEWAF phototoxic EC50 was 6.77 µM/L·mW∙s/cm2 (5.91-7.64
µM/L·mW∙s /cm2) (Figure 1D).
Weathered source CEWAF dilutions contained 0, 0.2, 0.9, 3.2, 12.9, and 49.9 µg/L
tPAH50. Both weathered source oil tests utilized two UV gradations (100% and 10%). Weathered
source CEWAF 100% UV exposures received an integrated dose of 2436 mW∙s/cm2 with a mean
intensity of 0.040 ± 0.019 mW/cm2/s. Significant toxicity was observed to occur only in the 49.9
µg/L tPAH50 exposures in the 100% UV treatment (p < 0.001) (Figure 2A). The artificially
weathered source oil CEWAF phototoxic EC50 was 14.7 µM/L·mW∙s/cm2 (no solution to 95%
confidence interval) (Figure 2B).
44
Weathered source HEWAF dilutions contained 0, 2.0, 4.0, 6.7, 18.6, 67.9 µg/L tPAH50.
Weathered source HEWAF 100% UV exposures received an integrated dose of 1754 mW·s/cm2
with a mean intensity of 0.031 ± 0.014 mW/cm2/s. Significant toxicity was observed at
exposures ≥ 4.0 µg/L tPAH50 in the 100% UV treatment, and ≥ 18.6 µg/L tPAH50 in the 10% UV
treatment (p < 0.001) (Figure 2C). The artificially weathered source oil HEWAF phototoxic EC50
was 2.16 µM/L·mW∙s/cm2 (1.52-2.79 µM/L·mW∙s/cm2) (Figure 2D).
45
Figure 1. Hatching success in mahi-mahi embryos exposed to field collected slick oil (A) CEWAF by tPAH50 concentration and UV
treatment, (B) CEWAF by phototoxic dose. (C) HEWAF by tPAH50 concentration and UV treatment, and (D) HEWAF by phototoxic
dose. Errors bars represent 1SE. Asterisks indicate treatments with mean percent hatch significantly different from controls.
46
Figure 2. Hatching success in mahi-mahi embryos exposed to artificially weathered source oil (A) CEWAF by tPAH50 concentration
and UV treatment, (B) CEWAF by phototoxic dose. (C) HEWAF by tPAH50 concentration and UV treatment, and (D) HEWAF by
phototoxic dose. Errors bars represent 1SE. Asterisks indicate treatments with mean percent hatch significantly different from
controls.
47
Discussion
In all four toxicity tests, toxicity as decreased hatching success occurred in a PAH and UV
dependent manner. Normal hatching time for mahi-mahi at 25°C is approximately 40 hours
post fertilization [30]. This suggests that embryos that did not hatch within a normal timeframe
(up to 48hrs in this study) are developmentally delayed following co-exposure to PAH and solar
radiation. This likely affects their potential for survival and recruitment compared to control
embryos. Concentrations of tPAH50 observed to result in photo-induced toxicity in these
experiments are well within the range of concentrations (0-84.8 µg/L) reported in the spill area
during the active phase of the 2010 Deepwater Horizon spill [31]. Measured tPAH50 values in
this study are based on samples taken immediately after WAF preparation and do not account
for loss of PAH over time in the exposure chambers. Exposure solutions were held static for the
duration of the toxicity test. Thus, the toxicity values reported here are likely conservative and
time-integrated effect values are likely lower.
Concentrations of PAH observed to result in toxicity in this study are also in agreement
with other literature-reported values using oil and marine species. Barron and Ka’aihue [9]
report an LC50 of 30 µg/L total PAH in a 96 h UV and PAH co-exposure to pacific Herring
embryos. Sellin-Jeffries et al. [19] induced significant mortality after 48 h at 15 µg/L anthracene
in pacific herring young of the year in field UV exposure tests, and at 5 µg/L anthracene in
laboratory tests using larvae and artificial UV. Duesterloh et al. [32] report a LC20 of
approximately 2 µg/L PAH in a single 4 h UV and PAH co-exposure to a marine calanoid
copepod. Oil exposures without a UV component report much higher median effect values.
Singer et al. [33] reported a range of LC50s (16.3-40.2 mg/L) in a series of larval topsmelt
48
exposures to crude oil. Pollino et al. [34] reported a range of LC50s (1.28 mg/L WAF, 14.5 mg/L
dispersant only, and 1.37 mg/L WAF and dispersant) in a series of WAF, dispersant, and WAF
with dispersant exposures to day-of-hatch rainbowfish larvae. Interestingly, the range of PAH
concentrations observed in this study to be acutely phototoxic under natural sunlight to
embryonic mahi are similar to concentrations observed to result in sublethal effects in pelagic
marine fish without UV. Mager et al. [21] reported significantly reduced critical swimming
speed in juvenile mahi-mahi that were exposed once, as embryos, to concentrations as low as
1.8 µg/L tPAH50. Incardona et al. [22] published similar findings, reporting pericardial edema
EC50s as low as 0.8 µg/L in tuna and 12.4 µg/L in amberjack.
Toxicity Associated with WAF Preparation Method
There was a significant reduction in photo-induced toxicity comparing CEWAF to
HEWAF from the same source oil. Dilutions of CEWAF made using artificially weathered oil were
approximately sevenfold less phototoxic than HEWAF counterparts. Similarly, CEWAF made
from more weathered slick oil was approximately threefold less phototoxic than slick oil
HEWAF. This implies that the reduction of photo-induced toxicity in CEWAFs could be related to
the degree of weathering the oil has undergone prior to addition of dispersant.
We have reported a similar finding in a previous study conducted using blue crab zoea
co-exposed to UV and WAF [10]. In that study, photo-induced toxicity was also reduced in
CEWAF preparations compared to HEWAF preparations. Investigations into dispersed oil
toxicity have reported preparations of oil and dispersant to be as toxic as oil alone [35], to
reduce toxicity compared to oil-only exposures [36], or to exhibit greater toxicity [37]. Reports
of increased bioaccumulation of PAHs with dispersant use would also be expected to increase
49
photo-induced toxicity [38, 39]. However, none of the cited studies investigated photo-induced
toxicity specifically as a mechanism. Dispersants may mediate photo-induced toxicity by some
other mechanism than altered bioavailability or bioaccumulation. Dispersants may have some
unknown effect on irradiation by UV, thus reducing the number of photochemical reactions at
the tissue level. Alternatively, dispersion may enhance photolysis and loss of PAH over time in
the exposure systems. Further investigation into the mechanism by which dispersants mediate
photo-induced toxicity is warranted as dispersants were widely utilized in the Deepwater
Horizon incident, as well as many other accidental oil releases.
Toxicity Associated with Oil Source
Oil source significantly influenced toxicity in HEWAF preparations as indicated by lack of
overlap in the phototoxic EC50 95% confidence intervals. HEWAF prepared from artificially
weathered source oil was more phototoxic (twofold) than HEWAF prepared from Slick A source
oil. This could be explained by analysis of the photodynamic PAH content of each preparation.
HEWAF stock prepared with artificially weathered source oil was calculated to have more than
double the anthracene equivalent of HEWAF stock prepared with slick oil, resulting in increased
toxic effect (Table 1). Interestingly, this could not be used to explain the lack of difference in
CEWAF. CEWAF stock prepared with artificially weathered source oil contained more than
twenty times the concentration of photodynamic PAHs than the CEWAF stock prepared with
slick oil. However, there was no difference in toxicity observed between the two. Furthermore,
CEWAF reduced toxicity on a tPAH50 basis when compared to HEWAF preparations of the same
source oil. We have previously reported similar findings in photo-induced toxicity tests with
blue crab zoea [10]. Taken together, these findings suggest that the mechanism by which
50
dispersant mediates photo-induced toxicity may be independent of photodynamic PAH
concentration.
The positive buoyancy of mahi-mahi embryos removes significant UV attenuation by the
water column as a factor in possible exposure scenarios. However, a variety of weather factors
can reduce the amount of UV that reaches the surface. Table 2 illustrates how photochemical
reciprocity shifts the concentration of PAH needed to produce the same phototoxic dose as UV
is reduced. Even with the lowest UV given in the table –requiring fourfold more PAH– the
concentrations calculated to for the EC20s range from 1.16-19.2 nM/L anthracene equivalent.
The latter of which is slightly less than the photodynamic PAH concentration in the highest
artificially weathered source HEWAF exposure in the present study. Thus, even under relatively
low UV conditions significant hatch failure could occur at the higher PAH concentrations
reported during the spill.
This study demonstrates that a UV component is important to a complete
understanding of the toxicity of PAHs to aquatic organisms, or hazard may be greatly
underestimated. Mahi-mahi and other pelagic fish species with similar life history traits may be
particularly vulnerable to photo-induced toxic effects. Their embryos are buoyant and
transparent, and newly hatched larvae remain close to the surface. This places them at risk for
UV exposure during all early life stages. Toxicity tests using Deepwater Horizon oil, but without
a UV component, have reported sublethal effects at low PAH concentrations (0.8-18.2 µg/L) in
mahi-mahi and other pelagic predatory fishes [21,22]. Effect concentrations determined in the
absence of UV may underestimate the toxicity of oil. It is possible that co-exposure to UV may
induce or exacerbate those sublethal effects at even lower concentrations of PAH.
51
Here, we have shown that co-exposure to slick oil from the Deepwater Horizon spill and
sunlight results in photo-induced toxicity in mahi-mahi embryos. Effects were observed well
within the range of tPAH50 concentrations reported during the spill and during relatively short
exposure periods (48 h) using WAF preparations both with and without dispersants. This study
demonstrates that photo-induced PAH toxicity likely contributed to overall toxic effects from
the Deepwater Horizon oil spill on early lifestage fish.
WAF Prep Type Oil type µM/L ANT equivalent
HEWAF Slick 0.79
HEWAF Artificially weathered source 1.75
CEWAF Slick 0.05
CEWAF Artificially weathered source 1.28
Table 1. Calculated anthracene equivalent concentrations from the four stock WAF
preparations. Concentrations presented in micromoles of anthracene equivalent per liter.
Integrated UV Dose
mWs/cm2
EC20 (ANT Equivalents)
nM/L (95% CI)
EC50 (ANT Equivalents)
nM/L (95% CI)
EC80 (ANT Equivalents) nM/L (95% CI)
Slick A 2423 1.68 (1.28-2.07) 2.79 (2.44-3.15) 4.66 (3.49-5.83)
HEWAF 1812 2.24 (1.72-2.77) 3.74 (3.26-4.22) 6.23 (4.66-7.79)
1214 3.35 (2.56-4.13) 5.58 (4.87-6.29) 9.29 (6.96-11.6)
607 6.70 (5.12-8.27) 11.2 (9.74-12.6) 18.6 (13.9-23.3)
WS 2423 0.289 (0.130-0.448) 0.891 (0.627-1.15) 2.74 (1.54-3.94)
HEWAF 1812 0.387 (0.174-0.600) 1.19 (0.839-1.54) 3.67 (2.06-5.27)
1214 0.578 (0.259-0.895) 1.78 (1.25-2.30) 5.48 (3.08-7.87)
607 1.16 (0.519-1.79) 3.56 (2.50-4.60) 11.0 (6.16-15.7)
Slick A 2423 1.95 (1.25-2.64) 4.87 (3.24-6.48) 12.1 (3.88-20.3)
CEWAF 1812 2.60 (1.67-3.53) 6.51 (4.33-8.66) 16.2 (5.19-27.1)
1214 3.89 (2.50-5.27) 9.72 (6.46-12.9) 24.1 (7.75-40.5)
52
607 7.78 (4.99-10.5) 19.4 (12.9-25.9) 48.3 (15.5-81.0)
WS 2423 4.81 (2.09-7.51) 6.06 (NA -13.7) 7.63 (NA-22.6)
CEWAF 1812 6.43 (2.80-10.0) 8.10 (NA-18.3) 10.2 (NA-30.2)
1214 9.60 (4.18-15.0) 12.1 (NA-27.3) 15.2 (NA-45.1) 607 19.2 (8.35-30.0) 24.2 (NA-54.5) 30.5 (NA-90.3)
Table 2. Calculated anthracene equivalent concentrations at the EC20, EC50, and EC80 and their
95% confidence intervals for four UV doses.
Acknowledgements
Data presented here are a subset of a larger toxicological database that is being
generated as part of the Deepwater Horizon Natural Resource Damage Assessment, therefore,
these data will be subject to additional analysis and interpretation which may include
interpretation in the context of additional data not presented here.
This work was supported as part of the Deepwater Horizon Natural Resource Damage
Assessment (NRDA). Data presented here are a subset of a larger toxicological database that is
being generated as part of the Deepwater Horizon NRDA, therefore, these data will be subject
to additional analysis and interpretation which may include interpretation in the context of
additional data not presented in this publication. The authors thank Stratus Consulting,
particularly Jeff Morris and Claire Lay, for their contributions.
53
References
1. Ankley GT, Burkhard LP, Cook PM, Diamond SA, Erickson RJ, Mount DR. 2003.
Assessing Risks from Photoactivated Toxicity of PAHs to Aquatic Organisms. Douben
PET Ed. PAHs: An Ecological Perspective, John Wiley & Sons Ltd. West Sussex,
England. pp 273-296.
2. Baumard P, Budzinski H, Garrigues P, Sorbe JC, Burgeot T, Bellocq J. 1998.
Concentrations of PAHs (polycyclic aromatic hydrocarbons) in various marine
organisms in relation to those in sediments and to trophic level. Mar. Pollut. Bull. 36
(12): 951-960.
3. Holst LL, Giesy JP. 1989. Chronic effects of the photoenhanced toxicity of anthracene
on Daphnia magna reproduction. Environ. Toxicol. Chem. 8(10): 933-942.
4. Diamond SA, Milroy NJ, Mattson VR, Heinis LJ, Mount DR. 2003. Photoactivated
toxicity in amphipods collected from polycyclic aromatic hydrocarbon–contaminated
sites. Environ. Toxicol. Chem. 22(11): 2752-2760.
5. Oris JT, Giesy Jr JP. 1987. The photo-induced toxicity of polycyclic aromatic
hydrocarbons to larvae of the fathead minnow (Pimephales promelas).
Chemosphere. 16(7): 1395-1404.
6. Newsted JL, Giesy JP. 1987. Predictive Models for Photoinduced Acute Toxicity of
Polycyclic Aromatic Hydrocarbons to Daphina magna, Strauss (Cladocera, crustacea).
Environ. Toxicol. Chem. 6: 445-461.
7. Atlas RM. 1975. Effects of temperature and crude oil composition on petroleum
biodegradation. Appl. Microbiol. 30(3): 396-403.
8. Peachey RL, Crosby DG. 1995. Ultraviolet Radiation and Coral Reefs. UNIHI Sea Grant
CR-95-03. Phototoxicity in a coral reef flat community. HIMB Report #41: 193-200..
9. Barron MG, Ka'aihue L. 2001. Potential for photoenhanced toxicity of spilled oil in
Prince William Sound and Gulf of Alaska waters. Mar. Pollut. Bull. 43(1): 86-92.
10. Alloy MM, Boube I, Griffitt RJ, Oris JT, Roberts AP. 2015. Photo-induced Toxicity of
Deepwater Horizon Slick Oil to Blue Crab (Callinectes sapidus) Larvae. Environ.
Toxicol. Chem. 34(9): 2061-2066.
11. Bowling JW, Leversee GJ, Landrum PF, Giesy JP. 1983. Acute mortality of
anthracene-contaminated fish exposed to sunlight. Aquat. Toxicol. 3(1): 79-90.
12. Boese BL, Lamberson JO, Swartz RC, Ozretich RJ. 1997. Photoinduced toxicity of
fluoranthene to seven marine benthic crustaceans. Arch. Environ. Contam. Toxicol.
32(4): 389-393.
13. Pelletier MC, Burgess RM, Ho KT, Kuhn A, McKinney RA, Ryba SA. 1997. Phototoxicity
of individual polycyclic aromatic hydrocarbons and petroleum to marine
invertebrate larvae and juveniles. Environ. Toxicol. Chem. 16(10): 2190-2199.
54
14. Cleveland L, Little EE, Calfee RD, Barron MG. 2000. Photoenhanced toxicity of
weathered oil to Mysidopsis bahia. Aquat. Toxicol. 49(1): 63-76.
15. Diamond SA, Mount DR, Mattson VR, Heinis LJ, Highland TL, Adams AD, Simcik MF.
2006. Photoactivated polycyclic aromatic hydrocarbon toxicity in medaka (Oryzias
latipes) embryos: relevance to environmental risk in contaminated sites. Environ.
Toxicol. Chem. 25(11): 3015-3023.
16. Hatch AC, Burton Jr GA. 1999. Photo-induced toxicity of PAHs to Hyalella azteca and
Chironomus tentans: effects of mixtures and behavior. Environ pollut. 106(2): 157-
167.
17. McNutt MK, Camilli R, Crone TJ, Guthrie GD, Hsieh PA, Ryerson TB, Savas O, Shaffer
F. 2012. Review of flow rate estimates of the Deepwater Horizon oil spill. Proc. Natl.
Acad. Sci. 109(50): 20260-20267.
18. Oris JT, Giesy JP. 1986. Photoinduced toxicity of anthracene to juvenile bluegill
sunfish (Lepomis macrochirus Rafinesque): Photoperiod effects and predictive
hazard evaluation. Environ. Toxicol. Chem. 5: 761-768.
19. Sellin-Jeffries MK, Claytor C, Stubblefield W, Pearson WH, Oris JT. 2013. Quantitative
Risk Model for Polycyclic Aromatic Hydrocarbon Photoinduced Toxicity in Pacific
Herring Following the Exxon Valdez Oil Spill. Environ. Sci. Technol. 47(10): 5450-
5458.
20. Willis AM, Oris JT. 2014. Acute photo-induced toxicity and toxicokinetics of single
compounds and mixtures of polycyclic aromatic hydrocarbons in zebrafish. Environ.
Toxicol. Chem. 33(9): 2028-2037.
21. Mager EM, Esbaugh AJ, Stieglitz JD, Hoenig R, Bodinier C, Incardona JP, Scholz NL,
Benetti DD, Grosell M. 2014. Acute embryonic or juvenile exposure to Deepwater
Horizon crude oil impairs the swimming performance of mahi-mahi (Coryphaena
hippurus). Environ. Sci. Technol. 45(12): 7053-7061.
22. Incardona JP, Gardner LD, Linbo TL, Brown TL, Esbaugh AJ, Mager EM, Stieglitz JD,
French BL, Labenia JS, Laetz CA, Tagal M, Sloan CA, Elizur A, Benetti DD, Grosell M,
Block BA, Scholz NL. 2014. Deepwater Horizon crude oil impacts the developing
hearts of large predatory pelagic fish. Proc. Natl. Acad. Sci USA. 111(15): E1510-
E1518.
23. Gibbs RH Jr, Collette BB. 1959. On the Identification, Distribution, and Biology of the
Dolphins, Coryphaena hippurus and C. equiselis. Bull. Mar. Sci. Gulf Caribbean. 9(2):
117-152.
24. NOAA Commercial Fisheries Statistics. [Cited 2014 May 10]. Available from:
http://www.st.nmfs.noaa.gov/commercial-fisheries/commercial-landings/annual-
landings/
55
25. Beardsley GL. 1967. Age, Growth, and Reproduction of the Dolphin, Coryphaena
hippurus, in the Straits of Florida. Copeia. (2): 441-451.
26. Stieglitz JD, Benetti DD, Hoenig RH, Sardenberg B, Welch AW, Miralao S. 2012.
Environmentally-conditioned, year-round volitional spawning of cobia (Rachycentron
canadum) in broodstock maturation systems. Aquac. Res. 43: 1557-1566.
27. Carls MG, Rice SD, Hose JE. 1998. Sensitivity of Fish Embryos to Weathered Crude
Oil: Part I. Low-Level Exposure During Incubation Causes Malformations, Genetic
Damage, and Mortality in Larval Pacific Herring (Clupea pallasi). Environ. Toxicol.
Chem. 18(3): 481-493.
28. SW-846 Manual for Waste Testing; United States Environmental Protection Agency:
Washington, DC, 1986; Vols. 1B and 1C, 8270D 1-72.
29. Ritz C, Streibig JC. 2005. Bioassay Analysis using R. J. Stat. Softw. 12(5): 1-22.
30. Ditty JG, Grimes CB, Cope JS. 1994. Larval development, distribution, and abundance
of common dolphin, Coryphaena hippurus, and pompano dolphin, C. equiselis
(family: Coryphaenidae), in the northern Gulf of Mexico. Fish. Bull. 92(2): 275-291.
31. Diercks AR, Highsmith RC, Asper VL, Joung D, Zhou Z, Guo L, Shiller AM, Joye SB,
Teske AP, Guinasso N, Wade TL, Lohrenz SE. 2010. Characterization of subsurface
polycyclic aromatic hydrocarbons at the Deepwater Horizon site. Geophys. Res. Lett.
37: L20602
32. Duesterloh S, Short JW, Barron MG. 2002. Photoenhanced Toxicity of Weathered
Alaska North Slope Cude Oil to the Calanoid Copepods Calanus marshallae and
Metridia okhotensis. Environ. Sci. Technol. 36: 3953-3959.
33. Singer MM, George S, Lee I, Jacobson S, Weetman LL, Blondina G, Tjeerdema RS,
Aurand D, Sowby ML. 1998. Effects of Dispersant Treatment on the Acute Toxicity of
Petroleum Hydrocarbons. Environ. Contam. Toxicol. 34: 177-187.
34. Pollino CA, Holdway DA. 2002. Toxicity Testing of Crude Oil and Related Compounds
Using Early Life Stages of the Crimson-Spotted Rainbowfish (Melanotaenia
fluviatilis). Ecotox. Environ. Safe. 52: 180-189.
35. Adams J, Sweezey M, Hodson PV. 2014. Oil and oil dispersant does not cause
synergistic toxicity to fish embryos. Environ. Toxicol. Chem. 33(1): 107-114.
36. Fuller C, Bonner J, Page C, Ernest A, McDonald T, McDonald S. 2004. Comparative
toxicity of oil, dispersant, and oil plus dispersant to several marine species. Environ.
Toxicol. Chem. 23(12): 2941-2949.
37. Kuhl AJ, Nyman JA, Kaller MD, Green CC. 2013. Dispersant and salinity effects on
weathering and acute toxicity of South Louisiana Crude oil. Environ. Toxicol. Chem.
32(11): 2611-2620.
38. Van Scoy AR, Voorhees J, Anderson BS, Philips BM, Tjeerdema RS. 2013. Use of
semipermeable membrane devices (SPMDs) to characterize dissolved hydrocarbon
56
fractions of both dispersed and undispersed oil. Environ. Sci. Process. Impacts. 15:
2016-2022.
39. Ramachandran SD, Hodson PV, Kahn CW, Lee K. 2004. Oil dispersant increases PAH
uptake by fish exposed to crude oil. Ecotox. Environ. Safe. 59: 300-308.
57
CHAPTER 4
SENSITIVITY OF EARLY LIFESTAGE RED DRUM (SCIAENOPS OCELLATUS) AND SPECKLED
SEATROUT (CYNOSCION NEBULOSUS) TO PHOTO–INDUCED TOXICITY OF NATURALLY
WEATHERED DEEPWATER HORIZON OIL
Introduction
Polycyclic aromatic hydrocarbons (PAHs) are a class of organic molecules with multiple
carbon rings. As a class, PAHs vary widely in toxicological and chemical properties [1]. In
general, PAHs are lipophilic [2]. PAHs exert toxicity through several mechanisms, however,
photo-induced or photo-enhanced toxicity often occurs at concentrations below the threshold
of other modes of toxicity [3-5]. Photo-induced toxicity is the phenomenon in which a
compound exhibits increased toxicity in the presence of certain wavelengths of light [5]. Effects
of PAH photo-induced toxicity include increased mortality [6-11], reduced fecundity [3],
delayed hatching [12] increased photo-avoidance behaviors [13, 5], and feeding inhibition [14].
The photo-induced toxicity of PAHs to aquatic species is well documented in the literature [5, 6,
11, 15-17].
On the 20th of April, 2010, the mobile offshore drilling unit Deepwater Horizon
experienced a series of events that resulted in the sinking of the vessel itself and subsequent
release of millions of barrels of oil from the wellhead unit until it was sealed on July 15th, 2010
[18]. Crude oil contains PAHs including those with photodynamic activity [19]. The Exxon Valdez
and Prestige oil spills are two examples where releases of oil resulted in potential photo-
induced PAH toxicity to early lifestage finfish [11,16, 20], shellfish [9, 12, 21], and marine
zooplankton [21].
58
Red drum (Sciaenops ocellatus) are found along the southern Atlantic and Gulf of
Mexico coasts [22]. It is an important commercial and recreational species. Commercial fishing
of red drum peaked in 1986 with nearly 15 million pounds caught [23]. Concerns about stock
depletion led to responses at the state and federal level to protect red drum populations,
including Executive Order 13449 in 2007, limiting the catch of red drum in federal waters [24].
Recreational fishing of red drum has increased since 1986 from 5 million pounds to more than
15 million pounds harvested in 2008 [23]. The mean catch between 2002 through 2011 for Gulf
of Mexico red drum was 8.9 million fish [23].
Red drum spawn in the open water neritic zone beginning in August and continuing into
December, however, regional variation in timing may shift this window by several weeks [22].
The number of eggs released per spawning event is dependent on female body size, varying in
laboratory conditions from two hundred thousand to in excess of two million eggs per female
[22]. Over the course of a single spawning season, a female may spawn every 2-4 days [25]. Red
drum larvae migrate with the tide into estuaries and settle in the cover of submerged
seagrasses [22].
Similarly, speckled seatrout (Cynoscion nebulosus) are distributed as far north as Virginia
and found along the shores of all Gulf of Mexico states [26]. The mean catch, combining harvest
and release, between 2002 through 2011 for Gulf of Mexico speckled seatrout was 29.9 million
fish [26]. Overfishing led to management responses and bans on several fishing methods in
order to allow for stocks to recover. Speckled seatrout spawn from April through October but,
again, this window of time varies regionally based on local conditions [26]. Speckled seatrout
spawn in a variety of habitats; they have been observed to spawn over submerged seagrass,
59
among floating masses of detritus, and in tidal areas with little or no vegetation present [26].
Spawning typically occurs in relatively shallow waters (3-4.6 m) [26]. Although older, larger
females spawn more frequently, over the course of a single season, a female may spawn every
2-9 days and release >1,000 eggs/g bodyweight [26]. Speckled seatrout larvae typically hatch in
estuarine habitat very close to their spawning area [26]. As larvae, they remain associated with
structure such as seagrass until they reach the juvenile life stage [26].
In both red drum and speckled seatrout, the eggs are buoyant, and larvae hatch in near
the surface where they are likely to encounter UV light. The goal of this study was to determine
the sensitivity of red drum and speckled seatrout larvae to photo-induced toxicity following
exposure to DWH spill oil. To accomplish this goal, larvae of both species were exposed to a
range of dilutions of two different field-collected oils and three gradations of UV. Data from this
study may be used as a component of the Deepwater Horizon Natural Resource Damage
Assessment (NRDA).
Materials and Methods
Test Organisms
Organisms were obtained from in house cultures at the Texas Parks and Wildlife Sea
Center (Lake Jackson, Texas, USA). Two species were tested, red drum and speckled seatrout.
Prior to use in bioassays, embryos were held until hatch (approximately 18-24 hpf). All
organisms used in tests were less than 48 hpf at the commencement of testing.
Test Solutions
Two oil samples collected in the field under chain of custody were used in these
experiments. Slick A is a surface slick oil collected on July 29, 2010 from the hold of barge
60
number CTC02404, which was receiving surface slick oil from various skimmer vessels
responding to the spill. Slick B is a more weathered surface slick oil collected on July 19, 2010 by
the skimmer vessel USCGC Juniper. Both of these oil samples are routinely used in testing as
part of the DWH NRDA. Filtered seawater from the Sea Center Hatchery (collected from a gulf
channel) was used in all control solutions and in preparation of treatment dilutions.
Stocks of high energy water accommodated fraction (HEWAF) of Slick A or Slick B were
prepared by mixing a known volume of water with a mass of slick oil (1g/L) in a Waring CB15
blender (Stamford, Connecticut), on low power, for thirty seconds. The mixture was transferred
to a separatory funnel and allowed to settle for one hour in darkness before sampling for PAH
analysis and utilization in test dilutions as described in Alloy et al. [11, 12]. Test dilutions were
prepared by dilution in filtered seawater to a nominal percentage of HEWAF. Samples of stocks
and dilutions were taken with every preparation and shipped (4°C) to ALS Environmental (Kelso,
Washington) for analysis. Fifty PAH analytes being used for NRDA analyses were quantified
using gas chromatography mass spectroscopy in single ion monitoring mode (GC/MS-SIM),
based on EPA method 8270D [27]. The sum concentrations of these 50 PAH analytes are
hereafter referred to as tPAH50.
Toxicity Tests
Larvae were exposed to one of a range of PAH concentrations combined with one of a
range of UV intensities in a fully factorial design for approximately 20 h. Exposures were
conducted in 250 mL borosilicate glass crystallizing dishes containing 10 larvae per dish. The
exposure period included an approximately 8 h equilibration period (under indoor low intensity
lighting), followed by a 7-h solar exposure, followed by a 5-h no-UV period before mortality was
61
assessed. Each bioassay had five PAH treatments with five replicate dishes per PAH treatment.
Tests were conducted with three UV (λ= 380nm) treatments (nominally 10%, 50%, and 100%
ambient natural sunlight).
Replicate dishes were suspended in an outdoor, flow-through water bath to maintain a
target temperature of 28°C. Dishes were floated in polystyrene foam insulation board with
holes cut to hold replicate dishes in contact with the temperature bath water across the
underside, and the majority of the sidewall. Sunlight was used as the source of UV radiation.
Screening materials were suspended over selected dishes to achieve treatment gradations of
UV. A specially formulated plastic sheet transparent to UV was used for a full intensity (100%
ambient) UV treatment (Professional Plastics, Fullerton, CA, USA). A metal mesh screen was
added over the top of the full intensity plastic as an additional, neutral density filter to achieve
an approximately 50% ambient UV treatment. A different formulation of plastic sheet allowing
transmission of < 10% of ambient UV (Professional Plastics, Fullerton, CA, USA) was used as a
control. UV was measured continuously during the exposures using a Biospherical BIC2104R
radiometer (BioSpherical Instruments, San Diego, CA).
Phototoxic Units
All tests were performed outdoors using ambient UV. Tests not performed in parallel
received different UV doses as a result. To account for differences in UV exposure, a phototoxic
unit was calculated using methods similar to Oris and Giesy [5] and previously described in Alloy
et al. (2015) [12]. Briefly, fourteen known phototoxic PAHs present in the WAF preparations
were used in the calculations: anthracene, benzo[a]anthracene, benzo[e]pyrene,
benzo[g,h,i]perylene, chrysene, fluoranthene, fluorene (as well as C1 and 2), phenanthrene (as
62
well as C1, 2, and 3), and pyrene. The aqueous concentration of each PAH was calculated as a
molar value and multiplied by its relative photodynamic activity (RPA) compared to anthracene
[5]. The sum of each of these values was used to calculate the sum concentration of anthracene
equivalents. UV doses are reported as the integration of the test duration at a resolution of one
second, expressed as mW∙s/cm2. The anthracene equivalent concentration is multiplied by the
integration of the UV irradiance at λ=380nm to produce the phototoxic dose.
Phototoxic dose =
Where ‘mW∙s’ refers to the integration of irradiance only at λ=380nm. Phototoxic units
are expressed as µM/L·mW∙s/cm2.
Statistical Analyses
For each toxicity test, percent survival data was arcsine-transformed to meet ANOVA
assumptions. A 2-factor analysis of variance (ANOVA) with a Dunnett’s post-hoc test was used
to determine differences in survival between treatments using UV treatment and tPAH50
concentration as factors. ANOVAs were performed using the statistical software JMP (version
11 SAS Institute, Cary, NC). Statistical significance was determined using α= 0.05. Median lethal
concentrations (LC50) for whole-test phototoxic dose, and individual UV treatments within
toxicity tests were calculated using the drc package in R (version 3.1.2) [28].
A table was generated of the anthracene equivalent molar concentrations required at a
given UV dose to meet three effect concentrations was generated using the mean UV intensity
of all tests, and the calculated lethal concentrations for twenty percent, fifty percent, and
eighty percent. The mean UV intensity was multiplied by an exposure duration of 7 hours. This
63
UV dose was used as the 100% UV exposure for the table, and was reduced accordingly for
75%, 50%, and 25% UV calculations.
Results
Red drum larvae were exposed to Slick A HEWAF dilutions containing 0.00, 1.46, 3.13,
5.67, and 11.76 µg/L tPAH50. Red drum exposed to the 100% UV treatment received a total
integrated dose of 705.79 mW•s/cm2 with a mean intensity (± 1SD) of 0.038 ± 0.021
mW/cm2/s. Mean survival of all treatments is detailed in Figure 1A. Significant mortality
occurred in the 100% UV treatment following exposure to tPAH50 concentrations ≥3.13 µg/L
(ANOVA, F(14,59)=11.42, Dunnett’s post-hoc p< 0.01). Median mortality tPAH50 concentrations
(LC50s) were calculated separately by UV treatment. The tPAH50 LC50 for the 50% UV and the
100% UV treatments were 12.2 µg/L tPAH50 (95% confidence interval = 7.37-17.0 µg/L tPAH50)
and 3.42 µg/L tPAH50 (95% confidence interval = 2.47-4.37 µg/L tPAH50). A model using
phototoxic units was also used to calculate a phototoxic LC50. The phototoxic LC50 for Slick A
HEWAF to red drum larvae was 1.41 µM/L•mW•s/cm2 (95% confidence interval = 1.17-1.65
µM/L•mW•s/cm2) (Figure 1B).
Red drum larvae were exposed to Slick B dilutions containing 0.00, 2.27, 5.11, and 8.25
µg/L tPAH50. 100% UV exposures of red drum larvae exposed to Slick B HEWAF received a total
integrated dose of 846.9 mW•s/cm2 with a mean intensity of 0.032 ± 0.015 mW/cm2/s. Mean
survival in all treatments is detailed in Figure 2A. Significant mortality occurred in the 50% and
100% UV treatments following exposure to tPAH50 concentrations ≥5.11 µg/L (ANVOA,
F(11,48)=80.47, Dunnett’s post-hoc p< 0.01) and ≥2.27 µg/L, respectively (Dunnett’s post-hoc p<
0.01). The tPAH50 LC50 in the 50% and 100% UV treatments were 5.79 µg/L tPAH50 (95%
64
confidence interval = 5.45-6.14 µg/L tPAH50) and 1.99 µg/L tPAH50 (95% confidence interval =
1.78-2.19 µg/L tPAH50), respectively. The phototoxic LC50 for Slick B to red drum larvae was 1.06
µM/L•mW•s/cm2 (95% confidence interval = 0.993-1.12 µM/L•mW•s/cm2) (Figure 2B).
Speckled seatrout larvae were exposed to Slick A dilutions which contained 0.00, 0.25,
0.43, 1.02, and 2.49 µg/L tPAH50. Speckled seatrout larvae in the 100% UV treatment exposed
to Slick A HEWAF received a total integrated dose of 1108.9 mW•s/cm2 with a mean intensity
of 0.042 ± 0.019 mW/cm2/s. Mean survival in all treatments is detailed in Figure 3A. Significant
mortality occurred at tPAH50 concentrations ≥2.40 µg/L in the 50% UV treatment (ANOVA,
F(14,60)=24.89, Dunnett’s post hoc p< 0.01), and ≥0.43 µg/L in the 100% UV treatment (Dunnett’s
post hoc p< 0.01). The tPAH50 LC50 in the 50% and 100% UV treatments was 2.41 µg/L tPAH50
(95% confidence interval = 0.741-4.07 µg/L tPAH50) and 0.827 µg/L tPAH50 (95% confidence
interval = 0.626-1.03 µg/L tPAH50), respectively. The phototoxic LC50 for Slick A to speckled
seatrout larvae was 0.516 µM/L•mW•s/cm2 (95% confidence interval = 0.478-0.553
µM/L•mW•s/cm2) (Figure 3B).
Speckled seatrout larvae were exposed to Slick B dilutions containing 0.00, 0.08, 0.18,
0.56, and 1.63 µg/L tPAH50. Speckled seatrout larvae in the 100% UV treatment exposed to
Slick B HEWAF received a total integrated dose of 1439.73 mW•s/cm2 with a mean intensity of
0.056 ± 0.019 mW/cm2/s. Mean survival in all treatments is detailed in Figure 4A. Significant
mortality occurred at 1.63 µg/L tPAH50 in the 50% UV treatment (ANOVA, F(14, 60)=26.53,
Dunnett’s post-hoc p< 0.01), and tPAH50 concentrations ≥0.18 µg/L in the 100% UV treatment
(Dunnett’s post-hoc p< 0.01). The tPAH50 LC50 in the 50% and 100% UV treatments were 1.01
µg/L tPAH50 (95% confidence interval = 0.802-1.21 µg/L tPAH50) and 0.182 ug/L tPAH50 (95%
65
confidence interval = 0.159-0.206 µg/L tPAH50), respectively. The phototoxic LC50 was 0.287
µM/L•mW•s/cm2 (95% confidence interval = 0.239-0.335 µM/L•mW•s/cm2) (Figure 4B).
66
Figure 1. [A] Mean percent mortality ±1 SE of larval red drum exposed to slick A HEWAF and one of three UV treatments. Asterisks indicate significant difference from control treatment of the same UV (α=0.05). [B] Phototoxic dose-response model of mortality in larval red drum exposed to slick A HEWAF and UV.
67
Figure 2. [A] Mean percent mortality ±1 SE of larval red drum exposed to slick B HEWAF and one of three UV treatments. Asterisks indicate significant difference from control treatment of the same UV (α=0.05). [B] Phototoxic dose-response model of mortality in larval red drum exposed to slick B HEWAF and UV.
68
Figure 3. [A] Mean percent mortality ±1 SE of larval speckled seatrout exposed to slick A HEWAF and one of three UV treatments. Asterisks indicate significant difference from control treatment of the same UV (α=0.05). [B] Phototoxic dose-response model of mortality in larval speckled seatrout exposed to slick A HEWAF and UV.
69
Figure 4. [A] Mean percent mortality ±1 SE of larval speckled seatrout exposed to slick B HEWAF and one of three UV treatments. Asterisks indicate significant difference from control treatment of the same UV (α=0.05). [B] Phototoxic dose-response model of mortality in larval speckled seatrout exposed to slick B HEWAF and UV.
70
Discussion
Co-exposure to natural sunlight increased the toxicity of DWH spill oil to larval red drum
and speckled seatrout in a tPAH50 and UV dose dependent manner. All calculated tPAH50 LC50s
(0.18-5.78 µg /L) in the present study are within the lower range of PAH concentrations (0-84.8
µg /L) reported in the DWH spill area [29]. Other photo-induced PAH toxicity tests, including
those using DWH spill oil, report total PAH EC50 or LC50 values that are within an order of
magnitude of those observed in the red drum and speckled seatrout tests [11, 12, 16, 20]. It is
worth noting that the tPAH50 values in this study are based on analysis of chemistry samples
taken immediately after WAF preparation and do not account for loss of PAH over time in the
actual exposures. Given that exposure solutions were not renewed for the duration of the
bioassay, the toxicity values reported here are likely higher than if we calculated them using
time-integrated doses due to the reduction in PAH concentration in the exposure solutions over
time.
The phototoxic LC50s (0.25-1.13 µM/L•mW•s/cm2) are substantially lower than those
reported in two similar studies on early lifestage mahi-mahi and blue crab [11, 12]. The
reported EC50s (phototoxic dose) for effects on hatching success in embryonic mahi-mahi were
between 6.8-11.8 µM/L•mW•s/cm2 (Slick A only). Median lethal concentrations (phototoxic
dose) reported for blue crab zoea were 9.5-20.6 µM/L•mW•s/cm2 (Slick A), and 9.9
µM/L•mW•s/cm2 (Slick B). While it is difficult to compare across taxa and lifestage, these data
suggest that red drum and speckled seatrout, both members of the drum family (Sciaenidae),
may be among the more sensitive test organisms to oil photo-induced toxicity. It is unlikely that
UV-sensitivity alone explains this result as survival in 10%, 50%, and 100% UV controls (no PAH)
71
was >90% in most cases. Regardless of mechanism, the sensitivity of larval red drum and
speckled seatrout lowers the range at which photo-induced PAH toxicity is observed among
Gulf of Mexico species.
Both red drum and speckled seatrout are estuarine species. This makes likely exposure
scenarios more complex than species that both spawn and live exclusively in open waters.
Immediately after hatching, red drum and speckled seatrout larvae at a similar age as those
used in this study can be found in both open and nearshore waters [25, 26]. In open water
areas of the Gulf of Mexico, UV-A Z10 (the depth at which only 10% of surface UV-A irradiance
remains) can be as deep as 37 m [31]. This suggests that, in open water areas, the likelihood for
co-exposure to PAH and UV is quite high. In coastal areas, UV attenuation varies greatly, and Z10
values as deep as 5 m and as shallow as <1 m have been reported [31]. Thus, the potential for
larvae to be exposed to UV in habitats where oil was trapped among seagrasses, salt marsh
vegetation, and sediments [30] may be more site- and season-specific. However, the sensitivity
of red drum and speckled seatrout larvae to oil photo-induced toxicity may result in significant
effects even when UV exposure is relatively low. For example, table 1 illustrates how
photochemical reciprocity shifts the concentration of PAH needed to produce the same
phototoxic dose as UV is reduced. The PAH doses required for median mortality under the
lowest UV given range from approximately 1.4-3.9 nM/L anthracene equivalent Thus, even
under relatively low UV conditions significant mortality could occur at the higher PAH
concentrations reported during the spill.
72
Co-exposure to UV as natural sunlight greatly increases the toxicity of DWH spill oil to
larval red drum and speckled seatrout. Effects were observed during short test durations (<24
h) and well within the range of tPAH50 concentrations reported during the spill. Data presented
here suggests that these two species may be among the most sensitive tested to date to oil
photo-induced toxicity. Significant toxicity was observed even under reduced (50% ambient) UV
intensity indicating that effects in the field may occur in more turbid, nearshore coastal waters
as well as highly transparent open water.
Integrated UV Dose LC20 (ANT Equivalents) LC50 (ANT Equivalents) LC80 (ANT Equivalents)
µWs/cm2 nM/L nM/L nM/L
RD 1065 0.279 (0.211-0.348) 0.988 (0.803-1.17) 3.49 (2.27-4.72) Slick A 800 0.372 (0.281-0.463) 1.31 (1.07-1.56) 4.65 (3.03-6.28)
533 0.558 (0.422-0.695) 1.97 (1.61-2.34) 6.98 (4.54-9.42) 266 1.12 (0.845-1.39) 3.96 (3.22-4.69) 14.0 (9.10-18.9)
RD 1065 0.622 (0.550-0.694) 0.951 (0.864-1.04) 1.45 (1.28-1.63) Slick B 800 0.828 (0.733-0.924) 1.27 (1.15-1.38) 1.93 (1.70-2.16)
533 1.24 (1.10-1.39) 1.90 (1.73-2.07) 2.90 (2.56-3.25) 266 2.49 (2.20-2.78) 3.81 (3.46-4.15) 5.82 (5.13-6.51)
SST 1065 0.412 (0.370-0.454) 0.626 (0.567-0.684) 0.950 (0.810-1.09) Slick A 800 0.549 (0.493-0.604) 0.833 (0.755-0.91) 1.26 (1.08-1.45)
533 0.823 (0.740-0.907) 1.25 (1.13-1.37) 1.90 (1.62-2.18) 266 1.65 (1.48-1.82) 2.50 (2.27-2.74) 3.80 (3.24-4.36)
SST 1065 0.166 (0.141-0.192) 0.349 (0.306-0.391) 0.730 (0.589-0.872) Slick B 800 0.221 (0.187-0.256) 0.464 (0.408-0.52) 0.972 (0.784-1.16)
533 0.332 (0.281-0.383) 0.696 (0.612-0.781) 1.46 (1.18-1.74) 266 0.666 (0.564-0.768) 1.40 (1.23-1.56) 2.92 (2.36-3.50)
Table 1. Calculated anthracene equivalent concentrations at the LC20, LC50, and LC80 and their
95% confidence intervals for four UV doses.
73
Acknowledgements
Data presented here are a subset of a larger toxicological database that is being
generated as part of the Deepwater Horizon Natural Resource Damage Assessment, therefore,
these data will be subject to additional analysis and interpretation which may include
interpretation in the context of additional data not presented here.
This work was supported as part of the Deepwater Horizon Natural Resource Damage
Assessment (NRDA). Data presented here are a subset of a larger toxicological database that is
being generated as part of the Deepwater Horizon NRDA, therefore, these data will be subject
to additional analysis and interpretation which may include interpretation in the context of
additional data not presented in this publication. Thanks to the Texas Parks and Wildlife’s Sea
Center for the use of their aquaculture facilities and providing test organisms.
74
References
1. Douben, PET. 2003. Assessing Risks from Photoactivated Toxicity of PAHs to Aquatic
Organisms. In PAHs: An Ecological Perspective; Gerald T. Ankley, Lawrence P.
Burkhard, Philip M. Cook, Stephen A. Diamond, Russell J. Erickson and David R.
Mount. John Wiley & Sons Ltd. West Sussex, England. pp 273-296.
2. Baumard P, Budzinski H, Garrigues P, Sorbe JC, Burgeot T, Bellocq J. 1998.
Concentrations of PAHs (polycyclic aromatic hydrocarbons) in various marine
organisms in relation to those in sediments and to trophic level. Marine Pollution
Bulletin, 36(12): 951-960.
3. Holst LL, Giesy JP. 1989. Chronic effects of the photoenhanced toxicity of anthracene
on Daphnia magna reproduction. Environmental Toxicology and Chemistry, 8(10):
933-942.
4. Diamond SA, Milroy NJ, Mattson VR, Heinis LJ, Mount DR. 2003. Photoactivated
toxicity in amphipods collected from polycyclic aromatic hydrocarbon–contaminated
sites. Environmental toxicology and chemistry, 22(11): 2752-2760.
5. Oris JT, Giesy JP. 1987. The photo-induced toxicity of polycyclic aromatic
hydrocarbons to larvae of the fathead minnow (Pimephales
promelas).Chemosphere, 16(7): 1395-1404.
6. Bowling JW, Leversee GJ, Landrum PF, Giesy JP. 1983. Acute mortality of
anthracene-contaminated fish exposed to sunlight. Aquatic Toxicology, 3(1): 79-90.
7. Boese BL, Lamberson JO, Swartz RC, Ozretich RJ. 1997. Photoinduced toxicity of
fluoranthene to seven marine benthic crustaceans.Archives of environmental
contamination and toxicology, 32(4): 389-393.
8. Pelletier MC, Burgess RM, Ho KT, Kuhn A, McKinney RA, Ryba SA. 1997. Phototoxicity
of individual polycyclic aromatic hydrocarbons and petroleum to marine
invertebrate larvae and juveniles. Environmental toxicology and chemistry, 16(10):
2190-2199.
9. Peachey RBJ. 2005. The synergism between hydrocarbon pollutants and UV
radiation: a potential link between coastal pollution and larval mortality. Journal of
Experimental Marine Biology and Ecology, 315: 103-114.
10. Cleveland L, Little EE, Calfee RD, Barron MG. 2000. Photoenhanced toxicity of
weathered oil to Mysidopsis bahia. Aquatic toxicology, 49(1): 63-76.
11. Alloy M, Baxter D, Stieglitz J, Mager E, Hoeing R, Benetti D, Grosell M, Oris J, Roberts
A. 2014. Ultraviolet Radiation Enhances the Toxicity of Deepwater Horizon Oil to
Mahi-mahi (Coryphaena hippurus) Embryos. Environmental Science and Technology
(in press).
75
12. Alloy MM, Boube I, Griffitt RJ, Oris JT, Roberts AP. 2014. Photo-induced Toxicity of
Deepwater Horizon Slick Oil to Blue Crab (Callinectes sapidus) Larvae. Environmental
Toxicology and Chemistry (in press).
13. Diamond SA, Mount DR, Mattson VR, Heinis LJ, Highland TL, Adams AD, Simcik MF.
2006. Photoactivated polycyclic aromatic hydrocarbon toxicity in medaka (Oryzias
latipes) embryos: relevance to environmental risk in contaminated
sites. Environmental toxicology and chemistry, 25(11): 3015-3023.
14. Hatch AC, Burton GA. 1999. Photo-induced toxicity of PAHs to Hyalella azteca and
Chironomus tentans: effects of mixtures and behavior. Environmental
pollution, 106(2): 157-167.
15. Oris JT, John PG. 1986. Photoinduced toxicity of anthracene to juvenile bluegill
sunfish (Lepomis macrochirus Rafinesque): Photoperiod effects and predictive
hazard evaluation. Environmental toxicology and chemistry 5.8: 761-768.
16. Sellin-Jeffries MK, Claytor C, Stubblefield W, Pearson WH, Oris JT. 2013. Quantitative
Risk Model for Polycyclic Aromatic Hydrocarbon Photoinduced Toxicity in Pacific
Herring Following the Exxon Valdez Oil Spill. Environmental science &
technology, 47(10): 5450-5458.
17. Willis AM, Oris JT. 2014. Acute photo-induced toxicity and toxicokinetics of single
compounds and mixtures of polycyclic aromatic hydrocarbons in zebrafish.
Environmental Toxicology & Chemistry, 33:9; 2028-2037
18. McNutt MK, Camilli R, Crone TJ, Guthrie GD, Hsieh PA, Ryerson TB, Savas O, Shaffer
F. 2012. Review of flow rate estimates of the Deepwater Horizon oil
spill. Proceedings of the National Academy of Sciences, 109(50): 20260-20267.
19. Atlas RM. 1975. Effects of temperature and crude oil composition on petroleum
biodegradation. Applied Microbiology, 30(3): 396-403.
20. Barron, M. G., Ka'aihue, L. 2001. Potential for photoenhanced toxicity of spilled oil in
Prince William Sound and Gulf of Alaska waters. Mar. Pollut. Bull. 43 (1) 86-92.
21. Saco-Álvarez, L, Bellas J, Nieto Ó, Bayona JM, Albaigés J, Beiras R. 2008. Toxicity and
phototoxicity of water-accommodated fraction obtained from Prestige fuel oil and
Marine fuel oil evaluated by marine bioassays. Science of the Total Environment,
394: 275-282.
22. National Marine Fisheries Service. 1986. Final Secretarial Fishery Management Plan
Regulatory Impact Review Regulatory Flexibility Analysis for the Red drum Fishery of
the Gulf of Mexico. National Oceanic and Atmospheric Administration.
23. Powers SP, Burns K. 2010. Summary Report of the Red drum Special Working Group
for the Gulf of Mexico Fishery Management Council. 1-7.
24. Executive Order 13449. 2007. Protection of Striped bass and Red Drum Fish
Populations. Federal Register 72(205): 60531-60532.
76
25. Wilson CA, Nieland DL. 1994. Reproductive biology of red drum, Sciaenops ocellatus,
from the neritic waters of the northern Gulf of Mexico. Fishery Bulletin 92: 841-850.
26. Blanchet H, Van Hoose M, McEachron L, Muller B, Warren J, Gill J, Waldrop T, Waller
J, Adams C, Ditton RB, Shively D, VanderKooy S. 2001. The Speckled Seatout Fishery
of the Gulf of Mexico, United States: A Regional Management Plan. Gulf States
Marine Fisheries Commission.
27. SW-846 Manual for Waste Testing; United States Environmental Protection Agency:
Washington, DC, 1986; Vols. 1B and 1C.
28. Ritz C, Streibig JC. 2005. Bioassay Analysis using R. Journal of Statistical Software.
12(5).
29. Diercks AR, Highsmith RC, Asper VL, Joung D, Zhou Z, Guo L, Shiller AM, Joye SB,
Teske AP, Guinasso N, Wade TL, Lohrenz SE. 2010. Characterization of subsurface
polycyclic aromatic hydrocarbons at the Deepwater Horizon site. Geophysical
Research Letters, 37: L20602
30. Michel J, Owens EH, Zengel S, Grahm A, Nixon Z, Allard T, Holton W, Reimer PD,
Lamarche A, White M, Rutherford N, Childs C, Mauseth G, Challenger G, Taylor E.
2013. Extent and Degree of Shoreline Oiling: Deepwater Horizon Oil Spill, Gulf of
Mexico, USA. PLOS one, 8(6): e65087 1-9.
31. Tedetti M, Sempere R. 2006. Penetration of Ultraviolet Radiation in the Marine
Environment. A review. Photochemistry and Photobiology. 82: 389-397.
32. Shank GC, Evans A. 2011. Distribution and photoreactivity of chromophoric dissolved
organic matter in northern Gulf of Mexico shelf waters. Continental Shelf Research,
31: 1128-1139.
77
CHAPTER 5
DISCUSSION
Influences on Polycyclic Aromatic Hydrocarbon Tissue Concentrations
Co-exposure of early lifestage organisms to polycyclic aromatic hydrocarbons (PAH) and
ultraviolet light (UV) resulted in photo-induced toxicity in all tested species. All species tested in
this work exhibit type III survivorship and rely on very large cohorts of offspring to produce
adequate recruitment. Significant reductions in organism success from photo-induced toxicity
could be deleterious to populations following PAH exposure. This study demonstrates that a UV
component is important to a complete understanding of the toxicity of PAHs to aquatic
organisms, or its environmental hazard may be greatly underestimated.
For photosensitization reactions to occur the organism must carry a body burden of
photo-dynamic PAHs and UV light of the correct range of wavelengths has to reach the cells
where the PAHs have partitioned to [1]. The uptake of PAHs in a natural system is complex and
modulated by various factors. Bioconcentration of PAHs also varies between species and taxa.
The blue crab represented crustacea in this work. Crustaceans are known to have larger
bioconcentration factors than fishes because of relatively poor PAH metabolism and excretion
compared to fishes. All other factors being equal, it would be expected that blue crab zoea
would be more sensitive to photo-induced toxicity than the other tested species because of a
greater accumulation of PAHs when exposed to equal waterborne concentrations. This was not
the case as blue crab were the least sensitive species of the four tested in this work. By the
same reasoning, it might be expected that mahi-mahi would take up similar body burdens to
78
red drum and speckled seatrout and thus exhibit very similar sensitivity of photo-induced PAH
toxicity. This was indeed the case between red drum and speckled seatrout, but not so with
mahi-mahi. Both red drum and speckled seatrout were exposed to PAHs for a shorter duration
than mahi-mahi but exhibited greater sensitivity. This may be due to the difference in the
lifestage of exposure between the three species. Red drum and speckled seatrout were both
exposed to PAHs as hatched larvae while mahi-mahi embryos spent the majority of their
exposure to both UV and PAHs within the protection of the egg chorion. It may be that the
mahi-mahi chorion hampers the partitioning of PAHs into the developing organism. Since there
were no renewals of test solutions the PAH exposure to the mahi-mahi may have been further
hampered by bacterial degradation and photolysis prior to hatch.
Another influence on PAH uptake and body burdens is the lipid fraction of the organism
in question. Lipids are the main partition compartment for PAHs in organisms [2, 3].
Composition of the organism is then important to its rate of uptake and final body burden at
equilibrium. Lipid content of early lifestage organisms can differ greatly from adults, especially
during yolk-dependent portions of development [4]. This can also vary throughout
development as some organisms hatch with little to no yolk left, e.g. blue crab zoea, while
others like mahi-mahi are dependent on it for longer durations after hatching. Prior to hatch, in
pelagic embryos, lipids can constitute as much as eighty percent of the embryo dry mass [4].
However, egg chorions often hamper movement of PAHs into the egg. This may reduce the
importance to lipid fraction to PAH uptake in pre-hatch fish exposure. In crab and a shrimp total
lipid constituted between two and one half percent up to ten percent of total wet mass [5, 6].
Fish larvae also vary in their total lipid composition by species. Rainuzzo et al. [7] reported lipid
79
composition at hatch to range from fourteen percent dry weight to twenty seven percent dry
weight among four fish species. So the lipid component of PAH partitioning into larvae would
be expected to be dependent on both the species and the developmental stage of the larvae in
question. This would imply that by relative expected lipid fractions the blue crab zoea would
have the lesser lipid fraction and thus body burden, making them less sensitive to photo-
induced PAH toxicity than fish larvae. This agrees with what was observed in testing between
blue crab and the red drum and speckled seatrout. However, by lipid fraction the mahi-mahi
embryos would likely have an equal or larger body burden of PAHs than the red drum and
speckled seatrout larvae as the larvae use up remaining yolk. In four fish species Rainuzzo et al.
[7] reported a reduction in lipid mass from the time of hatch to the time of first feeding,
although this reduction varied among the four species. As before, the difference between the
mahi-mahi embryonic tests and red drum and speckled seatrout larval tests may be attributable
once again to the relative impermeability of the chorion to PAHs. Additionally, lipid content is
more predicative of PAH body burdens for invertebrates than for fish species because fishes
readily metabolize PAHs [8]. However, recent studies have put forth that for very small bodied
organisms, such as those tested in this work, bioconcentration factors and lipid fraction may
not be as relevant as the waterborne exposure itself [2]. At these small masses the surface area
to volume ratio is such that direct diffusion into the organism is often the main form of gas
exchange and as a consequence PAH uptake. Following that viewpoint, post hatch exposure
might best be thought of as a combination of the dissolved concentration in the water and the
undissolved microdroplets and surface slick that comes into direct contact with the organism,
particularly gill surfaces.
80
Ultraviolet Wavelength Absorbing Pigmentation
The above assumes that differences in PAH partitioning and metabolism are the primary
factors influencing differences between species sensitivity to photo-induced PAH toxicity, which
may not be the case. UV exposure and sensitivity also determine a given species sensitivity. UV
protective environmental factors, organism behaviors and adaptations can have a great
influence on photo-induced toxic outcomes. However, the experimental design for this work
eliminated appreciable UV attenuation by water characteristics, and UV protective behaviors
such as vertical migration. This leaves only biochemical defenses to influence the absorbed UV
dose to the organism. Many of these biochemical defenses may also ameliorate reactive oxygen
species generation and damage.
Crustaceans accumulate carotenoids from their diet [9]. Carotenoids are known for
direct absorption of near UV wavelengths. These pigments are important to crustaceans in a
variety of metabolic functions and development [9]. As such the mother concentrates these
pigments into her developing eggs. Maternal transfer of these pigments into eggs gives the
hatched zoea a starting reserve prior to their first feeding event. Carotenoids are powerful
antioxidants and may offer some level of protection against ROS damage to zoea by that route.
This may have offered blue crab zoea both a level of UV protection that reduced PAH ROS
generation as well as protection against some amount of ROS that was generated despite UV
absorption. Because the zoea are entirely dependent on maternal transfer for these
carotenoids before their first feedings the variation between Slick A tests in blue crab might be
attributable to differences in maternal carotenoid supply.
81
Most marine fish species also accumulate dietary pigments as adults. However, the eggs
of the tested fish species are all transparent. Species such as red drum, speckled seatrout, and
the mahi-mahi disperse their eggs and provide no parental care. The primary defense against
predation for buoyant pelagic eggs is transparency throughout a very brief development period
before hatching. As a side effect, this permits high energy wavelengths of UV to pass freely
through the organism during development which could cause DNA damage. To manage this
many species pass on mycosporine-like amino acids (MAAs) and gadusol to their eggs [10].
These transparent compounds offer a range of protection against high energy, shorter
wavelength UV-B (peak absorbance varies by compound and typically ranges from 268 nm to
320 nm) while affording UV-A transparency as some predatory pelagic species’ vision extends
into the upper UV-A. These pigments do not absorb the UV-A range [11], which is most
responsible for photo-induced PAH toxicity. So that if mahi-mahi embyos were to absorb similar
PAH body burdens to blue crab zoea and then were exposed to similar UV conditions, it would
be expected that the mahi-mahi would be more sensitive than the blue crab because of the
photoprotective and antioxidant properties of their pigments over the MAAs and gadusol
available to the mahi-mahi. Something similar would be expected with red drum and speckled
seatrout larvae. Gadusols and MAA from development would remain in the developing larvae
but would still not afford significant protection against UV-A or ROS. In the absence of other
considerations this is consistent with the results of this work, blue crab were the least sensitive
larvae and speckled seatrout were the most sensitive.
Factors Relating to Species Sensitivity
82
Across all marine and freshwater species ultimate cause of mortality in PAH photo-
induced toxicity is the co-exposure of UV and photodynamic PAHs. However, the proximate
causes of mortality are loss of ion balance and asphyxiation. This is brought about by a chain of
events that ends with the destruction of the integumentary and gill surfaces of the organism.
Co-exposure of UV and photodynamic PAHs produces ROS, which lead to a lipid peroxidation
chain reaction in the cell membrane. This, in turn, leads to a loss of the cell’s osmoregulation
abilities which can result in apoptosis or necrosis. Tissues at the outer surface of the organism,
gill and integument, are subject to the most intense damage [12]. These are also the tissues
where most of the oxygen/carbon dioxide exchange occurs. In some small fish larvae the
majority of respiration happens by diffusion through the skin rather than across the gills.
Sufficient damage to these tissues removes the organisms’ ability to respire and asphyxiation
follows. In a photo-induced toxicity study focused on the effects on gills it has been observed
that several responses to damage contribute to the loss of ion balance and gas exchange
beyond direct destruction of gill tissue [12]. These were reported to include mucosal cell
hypertrophy, edema, and vasoconstriction [12]. These act to increase diffusion distances and to
hamper control of ion balance in both freshwater and marine organisms. In hyperosmotic
conditions this means elevated ion levels in the bloodstream and in hypoosmotic conditions
this means decreased ion levels in the bloodstream [13]. Organisms with great control over ion
balance can often be resistant to PAH toxicity by having more robust ion regulation capabilities.
The blue crab are known to have a greater range of hypoxia tolerance than mahi-mahi, the
former being able to survive in 16% oxygen saturation conditions while the latter has been
known to die >66% saturation conditions [14, 15]. There is a similar relationship with salinity
83
tolerance, mahi-mahi are able to tolerate lower salinities and fresh water for only brief periods
while the euryhaline blue crab can tolerate very low salinities and hypersaline conditions for
prolonged periods [16, 17]. This is not surprising as in their natural habitats only the blue crab
would normally see a wide range of salinities and low oxygen concentrations. The red drum and
speckled seatrout share similar habitat with the blue crab and also exhibit a wider range of
tolerance to hypoxic conditions and salinities than the mahi-mahi [18]. If the organisms in this
work were to be ordered by tolerance to hypoxia it would be expected that the blue crab would
be the most resistant to photo-induced PAH toxicity and the mahi-mahi the least. Yet the mahi-
mahi fall in the middle by phototoxic LC50. This could be explained by differences in lifestage
testing between embryos and larvae. Testing mahi-mahi larvae instead of embryos may yield
results more in line with the association of hypoxia tolerance as a predictor of resistance to
photo-induced PAH toxicity. Pigments in blue cab that absorb UV and act as antioxidants as well
as differing PAH metabolism in blue crab, as discussed above, may cloud the comparison. The
sheephead minnow (Cyprinodon variegatus) is an estuarine fish that was used in testing related
to this work. While not included in this body of work, testing on the sheepshead minnow
showed it to be very resistant to photo-induced PAH toxicity in comparison to the other tested
fishes. The sheephead minnow is an exceptional osmoregulator, known to be tolerant to
salinities ranging from 0 ppt to 142 ppt [19, 20]. Sheepshead were tested both as embryos and
as larvae. Larvae were shown to be more sensitive than embryos when exposed to overlapping
concentrations, however in both tests the phototoxic LC50 was an order of magnitude greater
than mahi-mahi embryos. Testing of more pelagic species and more estuarine species is
84
necessary to develop a more defined relationship between salinity and hypoxia tolerance and
resistance to photo-induced PAH toxicity.
Taking into account all of the discussed factors above it is not surprising that the blue
crab zoea were the least sensitive of the four tested species. The lower sensitivity of the mahi-
mahi compared to the red drum and speckled seatrout may be attributable to the protection of
the chorion through the majority of exposure. The origin of the differences in sensitivity
between the red drum and speckled seatrout is less clear at this time. Further testing might be
required to make the root causes clear. It is worth note that despite the protective factors in its
favor, the blue crab was still susceptible to photo-induced PAH toxicity at relatively low PAH
concentrations and with co-exposure to ambient sunlight.
Possible Effects on Recruitment
For the species tested in this work, and many type III survivorship marine organisms,
sufficient recruitment requires large spawns. Both eggs and young larvae are vulnerable to
predation, although predation pressure is thought to reduce as larvae grow. Hatched larvae are
also subject to starvation. A very generalized statement of pelagic spawning species is that
99.99% of fertilized embryos do not survive long enough to reach sexual maturity [21]. A
significant increase in mortality rate (M) from photo-induced PAH toxicity can have a
multiplicative reduction in overall recruitment [21]. For example, given a mahi-mahi spawn of
one million fertilized embryos the normal expectation would be that about one hundred would
reach sexual maturity. A five percent increase in the mortality rate would reduce one hundred
to sixty three. A ten percent increase in M would reduce the expected one hundred to forty. A
fifty percent increase in M would result in a one hundredfold reduction in expected
85
recruitment. However, this is an adjustment to M in absence of other factors already
contributing to M such as the availability of food. Early lifestage larvae such as those studied in
this work are dependent on zooplankton and their naupulii as a major food source. If photo-
induced PAH toxicity reduced the availability of these organisms to the fish and crab larvae
there would most likely be a greater increase to M than by considering direct mortality induced
by photo-induced PAH toxicity alone. This reduction in recruitment, even in the perhaps
unlikely absence of trophic cascade effects on adults, would adversely affect future
reproduction and recruitment. Just as larvae are dependent on zooplankton as a primary food
source, fingerling fish and pre-settlement megalopa crab depend on earlier lifestage organisms
of different species and even their own as prey. In this manner, significant reductions in larvae
hatching success and early survival could have deleterious effects to organisms not directly
affected by photo-induced PAH toxicity.
The hazard that photo-induced PAH toxicity presents to marine species is a complex
matter that varies by the physiological characteristics of the species, and their lifestage. Among
the species tested in this work sensitivity ranged across two orders of magnitude. Even the least
sensitive species, the blue crab, were shown to be vulnerable to relatively short duration
exposures. As representatives of the estuary, nearshore, and offshore habitats the tested
species demonstrate the possibility for photo-induced PAH toxicity to organisms that inhabit
these systems. Further testing on other representative species, particularly pelagics, is needed.
Factors that influence PAH concentration and UV penetration also must be taken into account
in an assessment of the environmental risk poised to species residing in these systems.
86
Acknowledgements
Data presented here are a subset of a larger toxicological database that is being
generated as part of the Deepwater Horizon Natural Resource Damage Assessment, therefore,
these data will be subject to additional analysis and interpretation which may include
interpretation in the context of additional data not presented here.
This work was supported as part of the Deepwater Horizon Natural Resource Damage
Assessment (NRDA). Data discussed here are a subset of a larger toxicological database that is
being generated as part of the Deepwater Horizon NRDA, therefore, these data will be subject
to additional analysis and interpretation which may include interpretation in the context of
additional data not presented in this work.
I thank my advisor, Dr. Aaron Roberts, for seeing me through two graduate degrees and
all the trials and tribulations that are inherent with the endeavor. I thank my committee for
their input, advice, guidance, and patience with the peculiarities involved with working
together with both government and consulting agencies. I thank my friends for their
understanding when I could only give them redacted explanations about my work these past
years. I thank my family for their unconditional support throughout my graduate career. I
thank NOAA and Stratus (Abt Associates) for this immense opportunity.
87
References
1. Diamond SA. 2003. Photoactivated Toxicity in Aquatic Environments. In Helbling EW,
Zagarese H, eds, UV Effects in Aquatic Organisms and Ecosystems. Vol–1
Comprehensive Series in Photochemistry & Photobiology. Cambridge Royal Society
of Chemistry, Cambridge, United Kingdom, pp 219-250.
2. Willis AM, Oris JT. 2014. Acute photo-induced toxicity and toxicokinetics of single
compounds and mixtures of polycyclic aromatic hydrocarbons in zebrafish. Environ
Toxicol Chem, 33(9): 2028-2037
3. Arnot JA, Gobas FAPC. 2006. A review of bioconcentration factor (BCF) and
bioaccumulation factor (BAF) assessments for organic chemicals in aquatic
organisms. Environ Rev. 14: 257-297
4. Kunz YW. 2004. Yolk (vitellus). In Developmental Biology of Teleost Fishes. Springer,
Netherlands, pp 23-40.
5. Torres G, Giménez L, Anger K. 2002. Effects of reduced salinity on the biochemical
composition (lipid, protein) of zoea 1 decapod crustacean larvae. J Exp Mar Biol Ecol.
277: 43-60
6. Palacios E, Racotta IS, Heras H, Marty Y, Moal J, Samain JF. 2002. Relation between
lipid and fatty acid composition of eggs and larval survival in white pacific shrimp
(Penaeus vannamei, Boone, 1931). Aquacult Int. 9(6): 531-543
7. Rainuzzo JR, Reitan KI, Jørgensen L. 1992. Comparative study on the fatty acid and
lipid composition of four marine fish larvae. Comp Biochem Phys. 103B(1): 21-26
8. Varanasi, Usha. Metabolism of polycyclic aromatic hydrocarbons in the aquatic
environment. CRC Press, 1989.
9. Liñán-Cabello MA, Paniagua-Michel J, Hopkins PM. 2002. Bioactive roles of
carotenoids and retinoids in crustaceans. Aquacult Nutr. 8: 299-309
10. Plack PA, Fraser NW, Grant PT, Middleton C, Mitchell AI, Thomson RH. 1981.
Gadusol, an enolic derivative of cyclohexane-1, 3-dione present in the roes of cod
and other marine fish: Isolation, properties and occurrence compared with ascorbic
acid. Biochem J. 199: 741-747
11. Dunlap WC, Shick JM. 1998. Ultraviolet Radiation-Absorbing Mycosporine-Like
Amino Acids in Coral Reef Organisms: a Biochemical and Environmental Perspective.
J Phycol. 34: 418-430.
12. Weinstein JE, Oris JT, Taylor DH. 1997. An ultrastructural examination of the mode of
UV-induced toxic action of fluoranthene in the fathead minnow, Pimephales
promelas. Aqua Toxicol. 39: 1-22
13. Engelhardt FR, Wong MP, Duey ME. 1981. Hydromineral balance and gill
morphology in rainbow trout Salmo gairdneri, acclimated to fresh and sea water, as
affected by petroleum exposure. Aquat Toxicol. 1: 175–186
88
14. Burnett LE, Stickle WB. 2001. Physiological responses to hypoxia. In Rabalais NN,
Turner RE. Eds, Coastal Hypoxia: Consequences for Living Resources and Ecosystems,
Coastal and Estuarine Studies, vol. 57. American Geophysical Union, Washington
D.C., pp. 101–114.
15. Lutnesky MMF, Szyper JP. 1990. Respiratory and behavioral responses of juvenile
dolphin fish to dissolved oxygen concentration. Prog Fish Cult. 52(3): 178-185
16. Waller U. 1989. Respiration and low oxygen tolerance of two fish species from the Arabian Sea, Cubiceps whiteleggi and Coryphaena hippurus. J Appl Ichthyol, 5: 141–150. doi: 10.1111/j.1439-0426.1989.tb00485.x
17. Tagatz ME. 1971. Osmoregulatory Ability of Blue Crabs in Different Temperature-Salinity Combinations. Chesapeak Sci. 12(1): 14-17
18. Holt J, Godbout RC, Arnold CR. 1981. Effects of temperature and salinity on egg hatching and larval survival of red drum, Sciaenops ocellata. Texas A & M University, Sea Grant College Program.
19. Nordlie FG. 1985. Osmotic regulation in the Sheepshead Minnow Cyprinodon variegates Lacépède. J Fish Biol. 26: 161–170. doi: 10.1111/j.1095-8649.1985.tb04253.x
20. Haney DC, Nordlie FG. 1997. Influence of Environmental Salinity on Routine Metabolic Rate and Critical Oxygen Tension of Cyprinodon variegatus. Physiol Zool. 70(5): 511-518
21. Beyer JE. 1989. Recruitment stability and survival – simple size-specific theory with examples from early life dynamics of marine fish. Dana. 7; 45-147