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Environmental chemicals modulate polar bear (Ursus maritimus) peroxisome proliferator-activated receptor gamma (PPARG) and adipogenesis in vitro Heli Routti, Roger Lille-Langøy, Mari Katrine Berg, Trine Fink, Mikael Harju, Kurt Kristiansen, Pawel Rostkowski, Marte Rusten, Ingebrigt Sylte, Lene Øygarden, and Anders Goksøyr Environ. Sci. Technol., Just Accepted Manuscript • DOI: 10.1021/acs.est.6b03020 • Publication Date (Web): 07 Sep 2016 Downloaded from http://pubs.acs.org on September 13, 2016
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Environmental chemicals modulate polar bear
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(Ursus maritimus) peroxisome proliferator-activated
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receptor gamma (PPARG) and adipogenesis in vitro
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Heli Routti *,†, Roger Lille-Langøy ‡, Mari K. Berg †,‡, Trine Fink §, Mikael Harju ||, Kurt
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Kristiansen ┴, Pawel Rostkowski ╡, Marte Rusten ‡,∇, Ingebrigt Sylte ┴, Lene Øygarden †,‡,
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Anders Goksøyr ‡
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† Norwegian Polar Institute, Fram Centre, 9296 Tromsø, Norway
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‡ Department of Biology, University of Bergen, 5020 Bergen, Norway
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§ Department of Health Science and Technology, Aalborg University, 9220 Aalborg, Denmark
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||
Norwegian Institute for Air Research, Fram Centre, 9296 Tromsø, Norway
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┴ Department of Medical Biology, Faculty of Health Sciences, UiT - The Arctic University of
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Norway, 9037 Tromsø, Norway
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╡ Norwegian Institute for Air Research, 2007 Kjeller, Norway
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ABSTRACT
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We studied interactions between polar bear peroxisome proliferator-activated receptor gamma
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(pbPPARG) and selected compounds using a luciferase reporter assay and predictions through
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molecular docking. Furthermore, we studied adipogenesis by liver and adipose tissue extracts
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from a polar bear and three synthetic mixtures of contaminants in murine 3T3-L1 preadipocytes
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and polar bear adipose tissue-derived stem cells (pbASCs). PCB153 and p,p’-DDE antagonized
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pbPPARG,
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tetrabromobisphenol A, and PCB170 had a weak agonistic effect on pbPPARG, while
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hexabromocyclododecane, bisphenol A, oxychlordane, and endosulfan were weak antagonists.
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pbPPARG-mediated luciferase activity was suppressed by synthetic contaminant mixtures
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reflecting levels measured in polar bear adipose tissue, as were transcript levels of PPARG and
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the PPARG target gene fatty acid binding protein 4 (FABP4) in pbASCs. Contaminant extracts
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from polar bear tissues enhanced triglyceride accumulation in murine 3T3-L1 cells and pbASCs,
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whereas triglyceride accumulation was not affected by the synthetic mixtures. Chemical
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characterization of extracts using non-target methods revealed presence of exogenous
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compounds that have previously been reported to induce adipogenesis. These compounds
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included phthalates, tonalide, and nonylphenol. In conclusion, major legacy contaminants in
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polar bear adipose tissue exert antagonistic effects on PPARG, but adipogenesis by a mixture
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containing emerging compounds may be enhanced through PPARG or other pathways.
although
their
predicted
receptor-ligand
affinity
was
weak.
PBDEs,
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INTRODUCTION
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The polar bear (Ursus maritimus) is an apex predator of arctic marine ecosystems that uses sea
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ice as a platform to hunt its prey, namely ringed seals.1 During ringed seal pupping and the
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moulting period in spring, polar bears feed excessively and accumulate energy reserves to
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survive periods with limited access to food.2 In the absence of sea ice, polar bears go through
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extensive fasting periods, which may be prolonged up to eight months combined with subsequent
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denning by pregnant females.2,3 During fasting periods polar bears depend almost entirely on
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energy stored in white adipose tissue.2,4
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White adipose tissue consists mainly of adipocytes, whose primary function is to store lipids in
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periods of excess of energy and mobilize lipids during energy deprivation.5,6 The process where
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undifferentiated mesenchymal cells differentiate into preadipocytes and further into lipid-filled
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adipocytes is called adipogenesis.5 Adipogenesis and promotion of lipid stores proceeds in two
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waves, as studied extensively using the murine 3T3-L1 preadipocyte cell line as a model.7,8 The
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first wave of adipogenesis is induced by an adipogenic cocktail and involves several
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transcription factors such as CCAAT/enhancer-binding protein (C/EBP) β and –δ, the
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glucocorticoid receptor, and the cAMP-response element binding protein (CREB). Furthermore,
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the first wave induces the second wave, during which the cells go through terminal
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differentiation through activation of the nuclear receptor peroxisome proliferator-activated
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receptor gamma (PPARG, NR1C1). PPARG, that forms a heterodimer with retinoic X receptor,
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is the major regulator of adipogenesis and promotion of lipid stores, but it also plays a role in
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other cell types such as macrophages, and several kidney and bone cell types.7 Endogenous
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PPARG agonists include fatty acids and their derivatives, and oxidized polyunsaturated lipids.9,10
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Polar bears’ ability to store enough energy and to survive during sea ice free periods is
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challenged by global climate change and decline of Arctic sea ice, which has already been linked
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to negative impacts on survival and reproduction.11 Another anthropogenic factor, namely
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pollution, may also affect polar bear energy homeostasis negatively. The polar bear is among the
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most polluted arctic species due to its position at the top of the Arctic marine food web.12,13 In
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particular, persistent organic pollutants (POPs), including polychlorinated biphenyls (PCBs),
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polybrominated diphenyl ethers (PBDEs), and chlorinated pesticides, as well as their
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metabolites, are found at high concentrations in polar bears.14 Because over 90% of the body
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burden of POPs in polar bears is stored in white adipose tissue,15 adipose tissue is at special risk
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for toxic effects of pollutants. Recent in vitro studies suggest that several POPs found in polar
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bear adipose tissue may affect adipogenesis in mice.16-18 In addition, other synthetic chemicals
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including organotins, and phthalates can activate PPARG, and many of them also induce
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adipogenesis in vitro and in vivo.18-22 Furthermore, several studies suggest associations between
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exposure to POPs among other endocrine disrupting chemicals with common metabolic
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problems in humans, such as obesity and type 2 diabetes.23-25
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We hypothesize that contaminants in polar bears may target PPARG and disrupt adipose tissue
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functions. The aim of this study was to study interactions between polar bear PPARG
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(pbPPARG) and selected contaminants at concentrations reflecting levels measured in polar bear
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adipose tissue; the contaminants as single compounds and in mixtures. In order to construct a
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transactivation assay, we cloned and sequenced pbPPARG from polar bear adipose tissue
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mRNA. Transactivation of pbPPARG was examined using a luciferase reporter assay. Ligand
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binding affinity was predicted by a docking and scoring strategy. Furthermore, we investigated
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the effect of both extracts and synthetic mixtures of POPs on the first and second wave of
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adipogenesis using 3T3-L1 cells. POPs in the extracts were quantified using target analyses
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whereas the presence of emerging and endogenous compounds was characterized using
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suspect/non-target analytical screening methods. We also established a method using polar bear
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adipose tissue-derived stem cells (pbASCs) to study adipogenesis by exposure to extracts and
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synthetic mixtures in these cells.
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EXPERIMENTAL
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Preparation of polar bear tissue extracts and synthetic mixtures
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Preparation of polar bear tissue extracts, quantification of POPs and subsequent preparation of
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synthetic mixtures is described in detail in supporting information. Briefly, contaminants were
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extracted from liver and adipose tissue from a healthy 10-year-old male bear from Svalbard,
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Norway. The samples were homogenized in dry Na2SO4, extracted with acetone/cyclohexane
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and cleaned by adding the lipid extracts onto a 30 cm long semipermeable membrane device.
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Further cleanup was achieved using a high performance liquid chromatography (HPLC) system
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utilizing gel permeation chromatography and a column packed with activated Florisil,
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fractionating the sample into three fractions. The first fraction contained neutral compounds such
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as PCBs, PBDEs and organochlorine pesticides, while the second and third fraction contained
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MeSO2-PCBs/DDE and hydroxylated (OH) PCBs/phenols, respectively. The volume of the final
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solvent, dimethyl sulphoxide (DMSO) was adjusted until the concentrations of the extracts were
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equivalent to 100 times the concentrations measured in polar bear tissues. Three separate
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synthetic mixtures including 1) 44 neutral POPs, 2) 10 neutral POPs, and 3) 16 MeSO2-
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metabolites of POPs were composed according to the concentrations and composition found in
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polar bear adipose tissue and dissolved in DMSO (Table S1). The mixture of 10 neutral POPs
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contained only compounds present at more than 0.1µM in the 44 neutral POP mixture.
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Suspect/Non-target screening
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Extracts of liver and adipose tissue were prepared for suspect/non-target screening and
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analyses were conducted by an ultra-high performance liquid chromatography system coupled to
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a high resolution quadrupole time-of flight mass spectrometer (Agilent 6550) as described in
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supporting information. The data was processed with various modules part of the Agilent Mass
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Hunter data processing platform (ver. B.07). The levels of confidence were set as previously
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proposed.26,27 Briefly, confidence level 1 means that the structure is confirmed by a reference
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standard. Level 2 refers to probable structure based on a library match and diagnostic evidence,
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and level 3 means that the structure is tentative. At confidence level 4 the molecular formula is
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unequivocal, whereas at confidence level 5 the compounds mass is of interest but there is no
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match with a reference standard or with a tentative candidate. We performed a systematic
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literature search to find out which compounds identified in the polar bear extracts have
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previously been reported to enhance adipogenesis. These compounds or closely related
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compounds were classified as “compounds of special interest” and we made a particular effort
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for improving their confidence level.
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Identification, cloning, and sequencing of polar bear PPARG
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Tissue sampling, RNA extraction, cDNA synthesis, and amplification of two distinct isoforms
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of pbPPARG cloned from liver and adipose tissue is described in supporting information. To
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evaluate the phylogeny of pbPPARG2 cloned from adipose tissue, nuclear receptor amino acid
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sequences were aligned using Clustal Omega.28
126 127
Luciferase reporter assay (LRA)
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Construction of a LRA plasmid encoding a fusion protein of the GAL4 DNA-binding domain
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(DBD) and the ligand-binding domain (LBD) of pbPPARG2 is described in detail in supporting
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information. Briefly, COS7 cells were transiently co-transfected with pCMX-GAL4-pbPPARG,
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tk(MH100)x4-luciferase, and pCMV-β-galactosidase at a mass ratio of 1:2:2 using the
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TransIT®-LT1 Transfection Reagent (Mirus Bio, Madison, WI, USA). The cells were exposed
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to test chemicals diluted in exposure medium for 24 hours. After exposure, the cells were lysed,
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and enzymatic activity was measured. Test compounds for agonistic effects included BDE28,
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BDE47, BDE99, BDE100, and BDE153, hexabromocyclododecane (HBCDD), bisphenol A
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(BPA), tetrabromobisphenol A (TBBPA), PCB118, PCB138, PCB153, PCB170, p,p’-DDE, and
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endosulfan. We assessed antagonistic effects of BPA, HBCDD, PCB-153, p,p’-DDE,
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oxychlordane, and endosulfan by exposing the cells to the test compounds in the presence of 0.5
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µM of a known PPARG ligand, rosiglitazone (Cayman Chemical, Tallinn, Estonia). We also
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tested agonistic and antagonistic effects of the mixture of neutral POPs, and the mixture of
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MeSO2-metabolites of POPs. Functionality of the LRA was established by exposure to
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rosiglitazone, and antagonists, bisphenol A diglycidylether (BADGE), and GW-9662 (Sigma
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Aldrich).29-31 All compounds for agonistic effects were tested in the range of (5 x 10-3) – 25 µM.
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Antagonistic effects were tested in the range of (9.6 x 10-3) – 50 µM. All compounds were
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dissolved in DMSO, and DMSO percentages were kept at 1% or below. In PPARG agonism and
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antagonism assays general cell viability was monitored through stability of β-galactosidase
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activities. To assess cell viability for antagonistic testing, we repeated the experiments in the
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presence of 10 µM of rosiglitazone. Potential toxicity of rosiglitazone was tested by Cytotoxicity
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detection kit LDH (LDH; Roche, Oslo, Norway). Effects of solvent (up to 2.5% DMSO) on the
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metabolic activity (CDFA-AM) and membrane integrity (resazurin reduction) of COS7 cells was
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perfomed.32
152 153
Modeling of PPARG-ligand interactions
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Polar bear PPARG ligand binding potential of environmental contaminants was studied using
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protein-ligand docking and scoring methods described in supporting information. Briefly, 3D X-
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ray structures of human PPARG (LBD 100% identical) in complex with structurally diverse
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ligands were used for docking into the LBD of pbPPARG. A molecular mechanical approach
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was used to calculate the potential for receptor binding of the test compounds to h/pbPPARG
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LBD. The virtual ligand screening scoring function was used to predict binding of test
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compounds to PPARG relative to data achieved for the ligands in the X-ray crystal structures.
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Test compounds with binding scores below -31 were considered as compounds with high
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putative binding affinities towards pbPPARG.
163 164 165
3T3-L1 differentiation assay
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Detailed methods for 3T3-L1 assay are described in supporting information. Briefly, to study
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how extracts and synthetic mixtures affect adipogenesis in 3T3-L1 cells through the first wave of
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the differentiation process,7 adipogenesis was carried out without the first-wave adipogenic
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mixture (isobutylmethylxanthine [IBMX], dexamethazone [DEX], and insulin). Effect of tissue
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extracts and synthetic mixtures on differentiation of 3T3-L1 cells through the first wave was
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determined after exposure to culture medium including 1 µg/ml insulin and test mixtures,
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DMSO, or rosiglitazone throughout a 10-day growth period. Contaminant extracts and synthetic
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mixtures dissolved in DMSO were diluted 1:100 (v/v) to Dulbecco´s Modified Eagle′s Medium
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(DMEM) to give a final concentration of contaminants in the culture medium equivalent to the
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concentrations found in polar bear tissues, and a solvent concentration of 1% (v/v). To
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investigate a dose-response effect, the contaminant mixtures were further diluted 1:3, 1:9, and
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1:27. The DMSO used for negative control in experiments with tissue extracts was subjected to
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the same extraction and clean-up steps as the polar bear tissue extracts. Rosiglitazone (1 µM in
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DMSO) was used as positive control. For our maximum adipogenic differentiation control, the
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culture medium given at day 0 contained 1 µg/ml insulin, 1 µM rosiglitazone, 500 µM IBMX
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and 1 µM DEX. The content of triglycerides in the 3T3-L1 cells was quantified
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spectrophotometrically (OD570nm, Adipogenesis Detection Kit Abcam, Cambridge, UK).
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Cytotoxicity was assessed by measuring the amount of lactate dehydrogenase released into the
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culture medium using Cytotoxicity Detection Kit Plus (LDH; Roche).
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Further, we studied the effect of synthetic mixtures on terminal differentiation, a process
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primarily driven by PPARG.7 Effect of synthetic mixtures of contaminants on terminal
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differentiation of 3T3-L1 cells was determined by OilRed O33 staining in cells given culture
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medium added adipogenic cocktail (500 µM IBMX, 250 nM DEX and 5 µg/ml insulin) at day 0,
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culture medium added 5 µg/ml insulin and the tested mixtures (or controls) at day 2 and culture
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medium during days 4-10. Synthetic mixtures gave a final concentration equivalent to
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concentrations in polar bear tissues, and a solvent concentration of 1% (v/v). To study dose-
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response relationships, the mixtures were further diluted 1:2 and 1:10.
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Adipogenic differentiation of polar bear adipose tissue-derived stem cells (pbASCs)
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Isolation, growth and establishment of suitable conditions for adipogenic differentiation of
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pbASCs are described in supporting information. pbASCs were seeded in 96-well plates at a
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density of 6400 cells/well (20,000 cells/cm2) and cultured to 100 % confluency (day -2). After
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two days adipogenic differentiation was induced in adipogenic medium (culture medium
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supplemented with 1 µg/mL insulin, 0.45 mM IBMX, 0.1 µM DEX), also containing the tested
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extract, synthetic mixture, or controls. The adipogenic media was changed day 3, 7 and 10. For
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exposures, the adipose tissue extract and the mixture of 10 neutral POPs in DMSO were diluted
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1:100 (v/v) in the adipogenic medium and the highest concentration in the medium was thus
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equivalent to the concentrations quantified in the polar bear adipose tissue (Table S1).
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Differentiation control cells were given 1 µM rosiglitazone while solvent control cells were
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given 1% (v/v) DMSO in addition to adipogenic medium. Undifferentiated control cells were
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maintained in basal medium (culture medium supplemented with 1 µg/mL insulin and 1%
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DMSO) without adipogenic medium. Experiments with synthetic mixtures at three different
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concentration levels were conducted using pbASCs originating from the two polar bears. They
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were seeded in triplicates, and the experiments were repeated twice. Due to a limited amount of
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extract, experiments with extract from polar bear adipose tissue were conducted at one
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concentration level using pbASCs from the 10 year male polar bear, and repeated three times.
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Controls were seeded in triplicates, while cells receiving the extracts were seeded in duplicates.
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At day 14, the accumulation of triglycerides in pbASCs was quantified spectrophotometically
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(OD570nm, Adipogenesis Detection Kit, Abcam).
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Transcriptional activity of PPARG and its target gene FABP4 was studied in pbASCs
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following exposure to the mixture of 10 neutral POPs for 14 days. Adipogenic differentiation of
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pbASCs was performed in 12-well plates and otherwise conducted as described above. Detailed
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methods are given in supporting information.
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Data analyses
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Statistical analysis was carried out using R version 3.2.2.34 Agonistic luciferase data were
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normalized over (divided by) solvent control (DMSO) and antagonistic data over positive control
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(0.5 µM rosiglitazone). Triglyceride levels in 3T3-L1 and pbASCs and transcript levels of
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PPARG and FABP4 were normalized over levels in solvent control.
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Effects of contaminants and their mixtures on transactivation of pbPPARG, transcriptional
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activity of PPARG and FABP4 in pbASCs and triglyceride accumulation in 3T3-L1 cells and
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pbASCs was investigated using linear models. Linear models were run separately for each
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compound/mixture. Exposure concentration was used as a categorical explanatory variable and
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each exposure concentration was compared to the control using treatment contrasts. The null
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hypothesis was rejected at α=0.05. Diagnostic plots of residuals were used to verify that the
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model assumptions were met (most importantly constant variance between residuals).35
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In one model for agonistic effects (BDE153) on pbPPARG transactivation the diagnostic plots
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of residuals revealed an outlier, which was omitted for further statistical analysis. The omittance
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of the one extreme value of BDE153 led to a significant positive effect at the 25 µM
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concentration, but the estimate was likely more robust without this outlier. Relative pbPPARG-
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mediated luciferase activity for agonistic and antagonistic effects were calculated from β(Cmax test
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compound)/
β(rosiglitazone) *100 and β(Cmax test compound)/ β(GW9662) *100, respectively. Relative triglyceride
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β(max
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accumulation was calculated from β(Cmax
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difference in fold change between the maximal concentration and the control based on linear
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models.
change)
*100.
β is the estimated
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Dose-response curves for transactivation of pbPPARG were calculated using R library drc
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version 2.5.12.36 The curves were fitted using a four parameter log-logistic model.36,37 To choose
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a best-fitting model for compounds showing >20% relative increase/decrease in luciferase
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activity compared to rosiglitazone/GW9662, we compared three models using a lack-of-fit F-
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test.38 These models included 1) a four parameter model, 2) a three parameter model where the
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upper plateau was fixed to the upper asymptote of rosiglitazone (agonistic effects) or the lower
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plateau to lower asymptote of GW9662 (antagonistic effects), and 3) a two parameter model
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where the lower and upper asymptotes were fixed to lower and upper plateaus of
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rosiglitazone/GW9662
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corresponding to a response midway between the estimates of the lower and upper plateaus
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(EC50 for agonist, IC50 for antagonist) were determined based on nonlinear least-squares
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estimates of the parameters of these models. EC/IC50 was calculated only for compounds
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showing
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rosiglitazone/GW9662. Dose-response models were also used to determine 20% of minimum
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response induced by known ligands.
>20%
for
relative
agonistic/antagonistic
increase/decrease
in
effects.
In
luciferase
addition,
activity
concentrations
compared
to
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RESULTS AND DISCUSSION
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Two PPARG isoforms in polar bears
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PPARG was cloned from liver and adipose tissue, and encoded to 475 and 505 amino acid
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(AA) proteins respectively (Figure S1). The shorter PPARG cloned from liver tissue (equivalent
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to hPPARG1), lacks the initial 30 AAs when compared to adipose tissue PPARG (equivalent to
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hPPARG2). This corresponds well to human PPARG, where the hPPARG1 is 28 AAs shorter
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than PPARG2. In many vertebrates, PPARG exists as at least two isoforms called PPARG1 and
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PPARG2. PPARG2 is expressed predominantly in adipose tissue as well as in macrophages,
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whereas PPARG1 is more widely expressed throughout the body.39,40 Of the two isoforms, the
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longer PPARG2 is expressed only at very low levels in liver.41 Compared to the PPARG coding
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sequence predicted from a polar bear genome sequencing (GenBank: XM_008697869)42, the
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longer adipose tissue PPARG lacked the initial 24 AA.
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Comparison of PPARG in polar bear to PPARG in other mammals revealed strong
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conservation, with overall AA identities of 98.2% (human), 99.6% (dog) and 97% (mouse)
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(Figure S2). The comparison of these PPARG orthologs confirms the variability of the N-
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terminal A/B-region, and the high degree of conservation (100%) of the DBD (C-region) and
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hinge (D-region). While the LBD of PPARG from human, dog, and polar bear was identical,
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three amino acids were substituted in the LBD of mouse PPARG. The high degree of
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conservation underlines the importance of this receptor and implies that PPARG orthologs would
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be expected to have similar activation patterns.
277 278
Validation of the transactivation assay
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For the ligand transactivation assay, we used the hinge and LBD domain of PPARG. Thus, the
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results from the assay should represent both the short and the long pbPPARG forms. In the
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GAL4-construct system, the risk of cross-reactivity by other cellular pathways is highly
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reduced,43 and we can thus assume that any activity we saw was due to the activation of
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pbPPARG-LBD and not nuclear receptors found endogenously in the cell. This assumption is
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supported by the results of the agonistic and antagonistic effects of known ligands on pbPPARG
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activation (Table 1, Figure S3). In the transiently transfected COS7 cells, luciferase activities
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increased approximately 8-fold when exposed to rosiglitazone, whereas rosiglitazone-induced
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(0.5 µM) luciferase production was inhibited by the known PPARG-antagonists GW9662 and
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BADGE (Table 1). EC50 and IC50 for rosiglitazone and GW9662 (Table 1) were comparable to
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previous studies using GAL4 systems.30,44,45 BADGE exposure led to a similar decrease of
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luciferase activity as GW9662, although at higher exposure concentrations (Table 1B, Figure
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S3B). This is in accordance with previous studies that have characterized BADGE as a low-
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affinity antagonist.29,46 Thus, the pbPPARG LRA appears to produce results comparable to those
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of previous studies.
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The relatively constant levels of β-galactosidase activities observed in cells exposed to
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different concentrations of test compounds (not shown), indicated that the rate of transcription
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and translation in the COS7 cells was unaffected by the exposures. At 1% and lower DMSO
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concentration, no significant reduction in metabolic activity (CDFA-AM) or membrane integrity
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(Resazurin reduction) was seen. Furthermore, antagonistic effects of test compounds were less
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pronounced in the presence of a higher concentration (10 µM) of rosiglitazone (results not
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shown). Thus, the viability of the cells appeared not to be severely affected by exposure of test
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compounds.
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Activation and predicted binding of polar bear PPARG by brominated compounds
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With the exception of bisphenol A and HBCDD, all the tested individual brominated
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compounds had a weak agonistic effect on pbPPARG (Table 1A, Figure S3A).. The most potent
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pbPPARG agonist in the test panel was TBBPA, which induced reporter gene transcription 2.5-
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fold at the highest exposure concentration, which was only about one fifth of the maximal
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activity induced by rosiglitazone (Table 1A). Of the other brominated flame retardants, all five
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PBDEs had weak agonistic activity on pbPPARG in our system and the most potent PBDE was
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BDE-47 (Table 1A). The measured agonistic effects of BDE47 and TBBPA are supported by
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previous studies which report induction of hPPARG by BDE47 and/or TBBPA in a similar
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system to ours and HEK293H cells stably expressing GAL4-PPARG-LBD.18,20 Furthermore,
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TBBPA had agonistic activity in stably-transfected HGELN-cells with full-length hPPARG.47
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Induction of hPPARG by BDE47 and TBBPA, but not BDE99 and BDE100 as shown in this
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study, has also been shown by using hPPARG-CALUX assay based on human osteosarcoma
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(U2OS) cell lines.48 Our results, as well as previous in vitro studies,18,20,48 refutes the hypothesis
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by Luthe et al.,49 which suggests that PBDEs would not interact with PPARs based on a
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theoretical structure-activity assessment.
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In contrast to the other brominated compounds tested in our study, BPA and HBCDD
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decreased pbPPARG-mediated luciferase activity induced by rosiglitazone (Table 1B, Figure
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S3B). In a previous study, no BPA-mediated human PPARG antagonism was observed.50 The
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discrepancy between the results may be related to detailed differences in experimental set-up.
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Docking of brominated compounds predicted weak receptor-ligand affinity for the brominated
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compound in this study (binding score < -31). This corresponds to previous in vitro and
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modeling studies which show that brominated compounds have weak binding potency to
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hPPARG LBD compared to rosiglitazone.47,51 Moreover, the results from the docking analysis
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were in agreement with the weak agonistic potential of brominated compounds demonstrated in
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the luciferase reporter gene assays.
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Activation and predicted binding of polar bear PPARG by chlorinated compounds
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The chlorinated compounds included in this study had very weak or no agonistic potential on
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pbPPARG, however, many of them had antagonistic properties towards pbPPARG (Table 1,
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Figure S3). PCB153 seems to be a full antagonist with similar efficacy but lower potency
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compared to that of GW9662 (Table 1B). Furthermore, PCB153 reduced the basal luciferase
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activity in the absence of rosiglitazone (Table 1A) which suggests that PCB153 is an inverse
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pbPPARG agonist
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luciferase reporter gene by PCB153 has also been observed in NIH-3T3 cells transfected with
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murine PPARG LBD coupled with GAL4.17 Exposure to PCB170 led to a weak increase in
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pbPPARG-induced luciferase activity (Table 1A). A similar tendency was also observed
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following PCB138 exposure. The different effects of PCB170 and PCB138 compared to PCB153
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may be due to their different chlorine-substitution patterns. PCB153 has no vicinal H-atoms,
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while PCB170 and PCB138 possess vicinal H-atoms in ortho-meta positions. Exposure to
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PCB118, the only tested PCB that easily acquires a planar configuration, did not lead to any
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significant changes in luciferase activity.
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in the luciferase reporter gene assay. Reduction of basal expression of the
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The chlorinated pesticides p,p’-DDE, oxychlordane and endosulfan showed antagonistic
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properties towards PPARG (Table 1B, Figure S3B,). p,p’-DDE appears to be a full antagonist
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with similar efficacy but lesser activity per dosing equivalent than GW9662 (Table 1B).
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Furthermore, and in contrast to PCB153, p,p’-DDE acted as a silent antagonist, as it did not
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reduce basal luciferase activity in absence of rosiglitazone (Table 1A). Oxychlordane partially
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decreased rosiglitazone-induced luciferase activity, the efficacy corresponding to one fourth of
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the maximal GW9662-induced inhibition (Table 1B). Endosulfan seemed to be a partial agonist
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(Table 1A) that also acted as a competitive antagonist in the presence of the full agonist
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rosiglitazone (Table 1B).
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Docking revealed that the chlorinated compounds which showed antagonistic activity did not
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show strong binding affinity towards pbPPARG LBD (score < -31). PPARG antagonism, as
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observed in our in vitro results, may be acquired through both covalent and weaker non-covalent
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modification of LBD.30,53,54 It is likely that most ligands interact with LBD through non-covalent
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interactions only. A molecule with a rigid and bulky distal phenyl, benzyl, or phenethyl
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substituent is important for non-covalent PPARG antagonist activity, which is strengthened to
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full antagonism by a chlorine substituent at the distal ring.54 These rigid molecules prevent helix
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12 to adopt an active state conformation53,55 which is needed for stable binding of ligand and
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recruitment of coactivators of PPARG.56 The full antagonists identified in our study, PCB153
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and p,p’-DDE, are both rigid bulky chlorine substituted molecules. This could explain their
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antagonistic potential towards pbPPARG in vitro, although they were not predicted as strong
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binders.
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Synthetic POP mixtures suppress polar bear PPARG
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Exposure to synthetic mixtures of neutral and MeSO2-POPs suppressed the activity of
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pbPPARG (Table 1B, Figure S3B). Relative inhibition at highest exposure concentration,
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corresponding to those identified in polar bear adipose tissue, was 30-50% of the maximal
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inhibition induced by GW9662 (Table 1B). Interestingly, the IC50 for the neutral 10 POP
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mixture was ~10 µM (concentration of summed compounds), which was slightly lower than the
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concentrations in adipose tissue of the male polar bear from Svalbard in which the mixture was
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based on (Table S1). However, 10 µM is within the range of average POP concentrations found
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in adipose tissue of polar bears from circumpolar subpopulations.14
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The inhibition at highest exposure concentrations was identical following exposure to the
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mixture of 44 and 10 neutral POPs. However, the inhibitory effect occurred at a lower
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concentration with the 44 compound mixture than with the 10 compound mixture (Figure S3B).
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The latter mixture contains only compounds present at >0.1 µM concentration in the 44 neutral
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POP mixture. This suggests that the compounds found at