These data are represented in the tables and graphs in the journal article, Antiandrogenic effects following multiple life stage exposure to the fungicide prochloraz in Xenopus laevis by JT Haselman et al. This dataset is associated with the following publication: Haselman, J., P. Kosian, J. Korte, A. Olmstead, and S. Degitz. Effects of multiple life stage exposure to the fungicide prochloraz in Xenopus laevis: Manifestations of antiandrogenic and other modes of toxicity. AQUATIC TOXICOLOGY. Elsevier Science Ltd, New York, NY, USA, 199: 240-251, (2018).

Dataset for "Degitz SJ, Degoey PP, Haselman JT, Olker JH, Stacy EH, Blanksma C, Meyer S, Mattingly KZ, Blackwell B, Opseth AS, Hornung MW. Evaluating potential developmental toxicity of perfluoroalkyl and polyfluoroalkyl substances in Xenopus laevis embryos and larvae. J Appl Toxicol. 2024 Mar 26. doi: 10.1002/jat.4599. Epub ahead of print. PMID: 38531109.". This dataset is associated with the following publication: Degitz, S., P. Degoey, J. Haselman, J. Olker, E. Stacy, C. Blanksma, S. Meyer, K. Mattingly, B. Blackwell, A. Opseth, and M. Hornung. Evaluating potential developmental toxicity of perfluoroalkyl and polyfluoroalkyl substances in Xenopus laevis embryos and larvae. JOURNAL OF APPLIED TOXICOLOGY. John Wiley & Sons, Ltd., Indianapolis, IN, USA, 44(7): 1040-1049, (2024).

This dataset shows the effects of herbicides and one fungicide (detected in Great Barrier Reef catchments) on the specific growth rates (from cell density data) of the microalgae Tisochrysis lutea during laboratory experiments conducted from 2018-2019. The aim of this project was to apply standard ecotoxicology protocols to determine the effects of Photosystem II (PSII), alternative herbicides and one fungicide on the growth of the marine microalgae Tisochrysis lutea. Growth bioassays were performed over 3-day exposures using pesticides that have been detected in the Great Barrier Reef catchment area (O'Brien et al., 2016). These toxicity data will enable improved assessment of the risks posed by PSII and alternative herbicides as well as the fungicide propiconazole to microalgae for both regulatory purposes and for comparison with other taxa. Methods: The haptophyte Tisochrysis lutea (formerly known as Isochrysis galbana)(Grant etal. 2017) (strain CS-177) was purchased from the Australian National Algae Supply Service, Hobart (CSIRO). Cultures of T. lutea were established in EDTA-free Guillard’s f/2 marine medium (Trenfield et al. 2015) (1 ml L-1 of f/2 medium in autoclaved natural seawater). Cultures were maintained in sterile 500 ml Erlenmeyer flasks as batch cultures in exponential growth phase with weekly aseptically transfers of 10 ml T. lutea suspension to 300 ml f/2 medium. Culture were maintained at 28 ± 1°C, 33 ± 1.5 psu and under a 12:12 h light:dark cycle (80 – 100 µmol photons m–2 s–1). Pesticide stock solutions were prepared using PESTANAL (Merck) analytical grade products (purity greater than or equal to 98%): diuron (CAS 330-54-1), metribuzin (CAS 21087-64-9), tebuthiuron (CAS 34014-18-1), bromacil (CAS 314-40-9), propazine (CAS 139-40-2), simazine (122-34-9), imazapic (CAS 104098-48-8), haloxyfop-p-methyl (CAS 72619-32-0), 2,4-D (CAS 94-75-7), MCPA (CAS 94-74-6), fluroxypyr (CAS 69377-81-7) and propiconazole (CAS 60207-90-1). The selection of pesticides was based on application rates and detection in coastal waters of the GBR (Grant et al. 2017, O’Brien et al. 2016). Pesticide stock solutions (100 – 1,000 mg L-1) were prepared by dissolving aliquots of the pure compounds in ultrapure water using clean, acid-washed (5% nitric acid) glass screw-top containers. Simazine, tebuthiuron and haloxyfop-p-methyl were dissolved using the carrier dimethyl sulfoxide (DMSO) (less than or equal to 0.02 % (v/v) in exposure solutions). Diuron, imazapic, metribuzin, bromacil, 2,4-D, propazine, MCPA, fluroxypyr and propiconazole were dissolved in acetone (less than or equal to 0.01 % (v/v) in exposure). Stock solutions were stored refrigerated and in the dark. Tests were conducted as previously described (Trenfield et al. 2015). Cultures of T. lutea were exposed to increasing concentrations of individual pesticides over a period of 72 h. Inoculum was taken from cultures in exponential growth phase (4-d old culture) and starting cell density assessed using a haemocytometer. For each treatment, a total volume of 250 mL test media was prepared in a clean, acid-washed 500 mL Schott bottle. Test media consisted of filtered (0.45 µm) seawater spiked with the respective pesticide stock, quarter strength EDTA-free f/2 media as nutrient source and T. lutea at a starting density of 3x103 or 1x104 cells mL-1. In each toxicity test, the response (specific growth rate of the culture) of the treatments exposed to pesticide were assessed against a seawater control group (no herbicide). For each test, 2 – 3 replicate 125 mL Erlenmeyer flasks (50 mL test volume) were assessed. Flasks were incubated at 27 – 29.0°C under a 12:12 h light:dark cycle (80 – 100 µmol photons m–2 s–1). After 72h, sub-samples (7 ml) were taken from each flask and cell densities measured using a flow cytometer (BD Accuri C6, BD Biosciences, CA, USA). Specific growth rates (SGR) were expressed as the logarithmic increase in cell density from day i (ti) to day j (tj) as per

Xenopus laevis tadpoles were held in 4 replicate vivaria for each of 4 treatments of neonicotinoid pesticides and one control treatment for at least one month (Control media, thiamethoxam high concentration of 100 ppm, thiamethoxam low concentrations of 20 ppm, clothianidin high concentrations of 100 ppm, and clothianidin low concentration of 20 ppm). Water was sampled for chemical testing on Day 33. Between Day 1 and 44, instantaneous measures of length were collected on a random selection of tadpoles from each vivarium. On Day 44, tadpole length (mm), weight, and developmental stage (Nieuwkoop-Faber staging) were measured for all tadpoles in all vivaria (three of the measured individuals from each replicate treatment group (total n=12 for each treatment) were vivisected and liver, brain, and somatic tissue frozen in RNA/DNA shield for qPCR analyses for another study). On Day 44, tadpoles (n=5) which had reached NF stage 57 were transferred to other vivaria and remained in their original treatment solution through Day 76; these animals were monitored until metamorphosis.

These data are from two studies conducted to evaluate the performance of the draft Larval Amphibian Growth and Development Assay for incorporation into the U.S. EPA's Endocrine Disruptor Screening Program Tier II testing battery. 4-tert-octylphenol was chosen as an environmental estrogenic compound and 17-beta-trenbolone was chosen as an environmental androgenic compound. Although the effects of these model environmental endocrine disruptors are not novel, these chemicals were used essentially as positive controls to represent each of the potential modes of toxicity that could be encountered by future unknown compounds ordered to be run through the LAGDA in support of risk assessment. Endpoints evaluated were larval growth and metamorphic development, blood thyroid hormone, thyroid histopathology, juvenile growth, juvenile histopathology of the liver, gonads, kidneys and reproductive ducts. This dataset is associated with the following publication: Haselman , J., P. Kosian , J. Korte , A. Olmstead, T. Iguchi, R. Johnson , and S. Degitz. Development of the larval amphibian growth and development assay: Effects of chronic 4-tert-octylphenol or 17ß-trenbolone exposure in Xenopus laevis from embryo to juvenile. JOURNAL OF APPLIED TOXICOLOGY. John Wiley & Sons, Ltd., Indianapolis, IN, USA, 36(12): 1639-1650, (2016).

This data covers reverse transcriptase qPCR quantification of microcystin gene activity during the summer bloom seasons in 2015, 2016 and 2017 for08/20/2019 Harsha Lake in Ohio. This dataset is associated with the following publication: Wymer, L., S. Vesper, I. Struewing, J. Allen, and J. Lu. Possible Antagonism between Cladosporium cladosporioides and Microcystis aeruginosa in a Freshwater Lake during Bloom Seasons. Life. MDPI, Basel, SWITZERLAND, 12(5): 742, (2022).

This dataset shows the effects of herbicides (detected in the Great Barrier Reef catchments) on the growth rates (from stem length and biomass) on the stonewort Ceratophyllum demersum during laboratory experiments conducted in 2019. The aims of this project were to develop and apply standard ecotoxicology protocols to determine the effects of non-PSII herbicides on the growth of the stonewort Ceratophyllum demersum. Growth bioassays were performed over 7-day exposures using herbicides that have been detected in the Great Barrier Reef catchment area (O’Brien et al. 2016). This toxicity data will enable improved assessment of the risks posed by non-PSII herbicides to aquatic macrophytes for both regulatory purposes and for comparison with other taxa. Methods: The stonewort Ceratophyllum demersum was supplied by Watergarden Paradise Aquatic Nursery, Bass Hill, NSW. Cultures were maintained in 500 L outdoor plastic tanks in recirculating dechlorinated tap water, aerated and maintained at ambient outdoor temperature and lighting. Test replicates selected 48 h in advance and acclimated in dechlorinated tap water, 26 ± 2 °C, under a 12:12 hr light:dark cycle (102 ± 9 µmol photons m–2 s–1). Herbicide stock solutions were prepared using PESTANAL (Sigma-Aldrich) analytical grade products (HPLC less than or equal to 98%): haloxyfop-p-methyl (CAS 72619-32-0), imazapic (CAS 104098-48-8) and triclopyr (CAS 5535-06-3). The selection of herbicides was based on application rates and detection in coastal waters of the GBR (Grant et al. 2017, O’Brien et al. 2016). Stock solutions were prepared in 500 mL glass volumetric flasks using milli-Q water. Haloxyfop-p-methyl was dissolved using analytical grade acetone (< 0.01% (v/v) in exposures). Imazapic was dissolved in methanol (less than or equal to 0.01% (v/v) in exposure). No solvent carrier was used for the preparation of triclopyr. Cultures of Ceratophyllum demersum were exposed to a range of herbicide concentrations over a period of 7 days. Plants were sourced from actively growing cultures free of overt disease or deformity. Individual plants approximately 35 mm long with 5 whorls and an apical tip were added to 150 mL of each herbicide solution concentration and control treatment. In each toxicity test, a control (no herbicide) and solvent control (if used) treatments were added to support the validity of the test protocols and to monitor continued performance of the assays. Experiments were conducted in autoclaved, recirculating dechlorinated tap water. Five replicates of each treatment solution and control were prepared and incubated at 26.6 ± 0.5 °C under a 12:12 h light:dark cycle (90 ± 6 µmol photons m–2 s–1). Each replicate treatment was photographed at a standard height to measure stem length at Day 0 and Day 7. Biomass of a representative numbers of fronds were weighed at Day 0 to 3 significant figures using an analytical balance after blotting for 15 seconds to remove excess moisture. Fronds from each treatment replicate were weighed at Day 7 using the same technique. Specific growth rates (SGR) were expressed as the logarithmic increase in stem length (mm) or biomass (g) from day i (ti) to day j (tj) as per equation (1), where SGRi-j is the specific growth rate from time i to j; Xj is the stem length or biomass at day j and Xi is the stem length or biomass at day i (OECD 2006). SGRi-j =[(ln Xj - ln X i) / (tj - ti)] (day-1) (1) SGR relative to the control / solvent control treatment was used to derive chronic effect values for growth inhibition. A test was considered valid, if the SGR for frond number or surface area of control replicates was greater than or equal to 0.0495 day-1 determined from (OECD 2006 and Riethmuller et al 2003). Physical and chemical characteristics of each treatment were measured at 0 and 7 days including pH, electrical conductivity and temperature. Temperature was also logged in 15-min intervals over the total test duration. Analytical samples were taken at

Data used for publication. This dataset is associated with the following publication: Struewing, K., P. Weaver, J. Lazorchak , B. Johnson , D. Funk, and D. Buckwalter. Part 2: Sensitivity comparisons of the insect Centroptilum triangulifer to Ceriodaphnia dubia and Daphnia magna using standard reference toxicants; NaCl, KCl and CuSO4. CHEMOSPHERE. Elsevier Science Ltd, New York, NY, USA, 11(139): 597-603, (2015).

Data files for "Oliver, S.K., Corsi, S.R., Baldwin, A.K., Nott, M.A., Ankley, G.T., Blackwell, B.R., Villeneuve, D.L., Hladik, M.L., Kolpin, D.W., Loken, L., DeCicco, L.A., Meyer, M.T. and Loftin, K.A. (2023), Pesticide Prioritization by Potential Biological Effects in Tributaries of the Laurentian Great Lakes. Environ Toxicol Chem, 42: 367-384. https://doi.org/10.1002/etc.5522". This dataset is associated with the following publication: Oliver, S., S. Corsi, A. Baldwin, M. Nott, G. Ankley, B. Blackwell, D. Villeneuve, M. Hladik, D. Kolpin, L. Loken, L. DeCicco, M. Meyer, and K. Loftin. Pesticide Prioritization by Potential Biological Effects in Tributaries of the Laurentian Great Lakes. ENVIRONMENTAL TOXICOLOGY AND CHEMISTRY. Society of Environmental Toxicology and Chemistry, Pensacola, FL, USA, 42(2): 367-384, (2023).

This dataset shows the effects of herbicides (detected in the Great Barrier Reef catchments) on growth rates (from surface area and biomass) and photosynthesis (effective quantum yield) on the aquatic fern Azolla pinnata during laboratory experiments conducted in 2019. The aims of this project were to develop and apply standard ecotoxicology protocols to determine the effects of Photosystem II (PSII) and alternative herbicides on the growth and photosynthetic efficiency of the aquatic fern Azolla pinnata. Growth bioassays were performed over 14-day exposures using herbicides that have been detected in the Great Barrier Reef catchment area (O’Brien et al. 2016). Chronic effects of herbicides on the photophysiology of A. pinnata, measured by chlorophyll fluorescence as the effective quantum yield (Delta F/Fm’) were investigated using PAM fluorometry after 14-day herbicide exposure. These toxicity data will enable improved assessment of the risks posed by PSII and alternative herbicides to aquatic macrophytes for both regulatory purposes and for comparison with other taxa. Methods: The aquatic fern Azolla pinnata was sourced from Watergarden Paradise Nursery, NSW. Cultures were established in IRRI2 medium (Pereira & Carrapiço 2009). Cultures were maintained in 10 L tubs containing 3–5 L IRRI2 as batch cultures with weekly transfers to fresh medium. Clean culture solutions were maintained at 26 ± 1 °C, under a 12:12 hr light:dark cycle (65-77µmol photons m–2 s–1). Herbicide stock solutions were prepared using PESTANAL (Sigma-Aldrich) analytical grade products (HPLC greater than or equal to 98%): diuron (CAS 330-54-1), fluometuron (CAS 2164-17-2), fluroxypyr (CAS 69377-81-7), haloxyfop-p-methyl (CAS 72619-32-0), imazapic (CAS 104098-48-8), isoxaflutole (CAS 141112-29-0) and triclopyr (CAS 5535-06-3). The selection of herbicides was based on application rates and detection in coastal waters of the GBR (Grant et al. 2017, O’Brien et al. 2016). Stock solutions were prepared in 100 mL glass volumetric flasks using milli-Q water. Diuron, haloxyfop-p-methyl and isoxaflutole were dissolved using analytical grade acetone (< 0.01% (v/v) in exposures). Imazapic was dissolved in methanol (less than 0.01% (v/v) in exposure). No solvent carrier was used for the preparation of the remaining herbicide stock solutions. Cultures of A. pinnata were exposed to a range of herbicide concentrations over a period of 14 days. Fronds were selected from actively growing cultures free of overt disease or deformity. Four triplicate fronds each comprising eight ramets were added to 100 mL of each herbicide solution concentration and control treatment. In each toxicity test, control (no herbicide) and solvent control (if used) treatments were added to support the validity of the test protocols and to monitor continued performance of the assays. Experiments were conducted in IRRI2 medium (Pereira & Carrapiço 2009) with solutions replaced at Day 7. Three replicates of each treatment solution and control were prepared and incubated at 26.6 ± 0.5 °C under a 12:12 h light:dark cycle (90 ± 6 µmol photons m–2 s–1). Each replicate treatment was photographed at a standard height to estimate surface area at Day 0 and Day 14. Biomass of a representative numbers of fronds were weighed to 4 significant figures using an analytical balance after blotting for 15 seconds to remove excess moisture. Fronds from each treatment replicate were weighed at Day 14 using the same technique. Specific growth rates (SGR) were expressed as the logarithmic increase in surface area or biomass from day i (ti) to day j (tj) as per equation (1), where SGRi-j is the specific growth rate from time i to j; Xj is the surface area or biomass at day j and Xi is the surface area or biomass at day i (OECD 2006). SGR i-j = [(ln Xj - ln Xi )/(tj - ti )] (day-1) SGR relative to the control / solvent control treatment was used to derive chronic effect values for growth inhibition. A test was considered