Research paperAn aryl hydrocarbon receptor from the caecilian Gymnopis multiplicata suggests low dioxin affinity in the ancestor of all three amphibian orders
Graphical abstract
Introduction
The aryl hydrocarbon receptor (AHR), a member of the Per-ARNT-Sim (bHLH/PAS) family of proteins (McIntosh et al., 2010), is a ligand-activated transcription factor that mediates the toxicity of a wide range of environmental contaminants, including chlorinated dioxin-like compounds and polynuclear aromatic hydrocarbons (Denison et al., 2011). The unliganded receptor is part of a cytoplasmic complex with hsp90, p23, and AIP (Murray and Perdew, 2011). Agonist binding triggers translocation to the nucleus, shedding of these chaperones, and dimerization with the ARNT protein. The AHR:ARNT heterodimer binds to cognate enhancer sequences (Seok et al., 2017) and alters transcription of numerous target genes (Frueh et al., 2001, Puga et al., 2000). Well-known gene targets include the “AHR gene battery,” encoding phase I and phase II detoxification enzymes such as the cytochrome P450 family 1 members (CYP1s) and UDP glucuronosyltransferase, glutathione S transferase, and quinone reductase (Nebert et al., 2000). Induced over two orders of magnitude, CYP1s are frequently used as a biomarker of exposure to AHR agonists (Hahn, 2002). AHR also exerts biological effects through “non-classical” mechanisms involving interactions with additional signaling pathways and nuclear proteins (Denison et al., 2011).
AHR can be activated by structurally diverse agonists of both xenobiotic and endogenous origin. The prototypical agonist in mechanistic toxicological studies of AHR is the industrial contaminant 2,3,7,8-tetrachlorodibenzo-p-dioxin (TCDD, dioxin). Among the most toxic of the planar halogenated aromatic hydrocarbons, TCDD binds vertebrate AHRs with relatively high affinity (Van den Berg et al., 2006). Another potent AHR agonist, 6-formylindolo[3,2-b]carbazole (FICZ), has endogenous sources, forming in vivo from tryptophan as a photoproduct, an oxidation product, or as a metabolite produced by gut bacteria (Rannug and Rannug, 2018). FICZ binds AHR with even higher affinity than TCDD, but it is rapidly metabolized by the detoxification enzymes induced by exposure (Wincent et al., 2009).
Dioxin toxicity varies substantially between different vertebrate species or populations. Many studies link differences in AHR ligand binding affinity to these variations. Invertebrate AHRs typically do not bind TCDD, and the animals are largely insensitive to its toxic effects (Hahn et al., 2017). TCDD-sensitive mouse strains express the high-affinity AHRb-1 allele, while toxicity is lower in strains expressing AHRd, which encodes a protein that binds TCDD with 4- to 10-fold lower affinity, comparable to the human receptor (Ema et al., 1994, Poland et al., 1994, Ramadoss and Perdew, 2004). Differential affinity for AHR also underlies wide-ranging variations in TCDD toxicity between many bird species (Farmahin et al., 2013, Karchner et al., 2006). Amphibian receptors display less robust xenobiotic binding (Lavine et al., 2005, Shoots et al., 2015), with X. laevis AHRs exhibiting Kd values for TCDD 20- to 50-fold higher than those of many fish, birds, and mammals (Karchner et al., 2005, Karchner et al., 2006). Amphibians are concomitantly much less sensitive to toxicity of dioxin-like chemicals (Beatty et al., 1976, Collier et al., 2008, Jung and Walker, 1997, Pezdirc et al., 2011, Vajda and Norris, 2005) and PAHs (Fort et al., 1989, Propst et al., 1997).
To elucidate the structural basis for differences in TCDD affinity, ligand-binding domains (LBDs) have been characterized in AHRs from animals across the spectrum of TCDD sensitivity. A comparative study of AHR1 from the chicken (Gallus gallus) and common tern (Sterna hirundo) identified two residues—I324 and S380—that are critical for high-affinity binding by the receptor from chicken, the species more sensitive to TCDD toxicity (Karchner et al., 2006). In mice, a single polymorphism (A375V) reduces TCDD affinity 4–5 fold in the AHRd allele vs. AHRb-1; the LBD from human AHR contains valine at the homologous position (Ema et al., 1994, Poland et al., 1994, Ramadoss and Perdew, 2004). Additional signature residues conferring high-affinity binding in mouse AHR (Pandini et al., 2009) and AHRs from other species (Fraccalvieri et al., 2013) were identified by homology modeling and confirmed using site-directed mutagenesis. Similar approaches were employed to explain the low TCDD affinity of amphibian AHRs. Three amino acids within the LBD of X. laevis AHR1β confer low-affinity binding—N325, A354, and A370 (Odio et al., 2013). Homologous residues are present in AHR from X. tropicalis (Order Anura; frogs and toads) and Ambystoma mexicanum (Order Caudata; salamanders; (Shoots et al., 2015). These shared sequence elements and functional properties suggest that low TCDD affinity emerged in the common ancestor of these two extant amphibian groups. Is it possible that low TCDD affinity appeared even earlier in amphibian evolution?
Caecilians, the legless amphibians, comprise Order Gymnophiona, the earliest of the extant orders to diverge from the common lineage (Hay et al., 1995, Pyron and Wiens, 2011, Zardoya and Meyer, 2001, Zhang and Wake, 2009, Zhang et al., 2005). Therefore, caecilians offer an opportunity to probe the timing of emergence of low affinity AHRs during amphibian evolution. If the caecilians possess a low-affinity AHR, then this phenotype likely arose in an ancestor of all extant groups. Alternatively, if caecilian AHRs bind dioxin-like compounds with high affinity—similar to AHRs from both previously- and more recently-derived vertebrate groups—then low-affinity binding must have evolved in the common ancestor of frogs and salamanders after the caecilian divergence. This study sought to address this question. In this first characterization of a caecilian AHR, we report the sequence, pharmacological properties, and a structural model of the ligand-binding domain of a receptor derived from Gymnopis multiplicata (the Varagua caecilian). Comparative studies of low-affinity amphibian AHRs will help discern the pleiotropic roles of AHR in development, physiology, and toxicology from both general and taxon-specific perspectives.
Section snippets
AHR ligands
TCDD was obtained from ULTRA Scientific dissolved in toluene. This material was dried under a N2 stream, dissolved in DMSO, and stored at room temperature. 6-formylindolo[3,2-b]carbazole (FICZ; Enzo Life Sciences; lyophilized powder) was dissolved in DMSO and stored in the dark at −20 °C.
cDNA cloning
Total RNA was extracted from a Gymnopis multiplicata tissue sample provided by the Museum of Vertebrate Zoology at the University of California, Berkeley using RNA STAT-60 (Tel-Test, Inc.). The sample, a
Sequence analysis of G. Multiplicata AHR
We determined the cDNA sequence of an AHR from Gymnopis multiplicata (the Varagua caecilian) using RT-PCR with degenerate primers and RACE PCR. The corresponding 3,742 nt mRNA contains an open reading frame of 2,532 nt, encoding an 843 residue polypeptide with predicted molecular mass of 92.7 kDa. The sequence is publicly available in the Genbank database with accession number MH457176. Sharing 59–66% identities with a wide range of tetrapod AHRs, the identification of this amino acid sequence
Conservation of low dioxin affinity in diverse amphibian AHRs
Previous characterizations of xenobiotic toxicity in amphibians reveal that frogs and salamanders are generally insensitive to the toxicity of dioxin-like chemicals (Beatty et al., 1976, Collier et al., 2008, Jung and Walker, 1997, Pezdirc et al., 2011, Vajda and Norris, 2005). Low-affinity agonist binding by their AHRs is likely a major mechanistic contributor to this phenotype (Lavine et al., 2005, Odio et al., 2013, Shoots et al., 2015). In this regard, these animals differ from both
CRediT authorship contribution statement
Sarah A. Kazzaz: Conceptualization, Methodology, Investigation, Visualization, Writing - original draft. Sara Giani Tagliabue: Methodology, Investigation, Formal analysis, Visualization, Writing - review & editing. Diana G. Franks: Methodology, Investigation. Michael S. Denison: Methodology, Writing - review & editing, Funding acquisition. Mark E. Hahn: Methodology, Supervision, Resources, Writing - review & editing, Funding acquisition Laura Bonati: Methodology, Formal analysis, Supervision,
Acknowledgements
We thank the Museum of Vertebrate Zoology at the University of California, Berkeley (Dr. Carol A. Spencer, Staff Curator of Herpetology) for providing the tissue sample from Gymnopis multiplicata. We thank Scott Freeburg for expert technical support and Kathy Gillen for critically reading the manuscript.
Funding statement
This work was funded by the National Institute of Environmental Health Sciences: R15 ES011130 (WHP), R01 ES07685 (MSD), R01 ES006272 and P42 ES007381 (MEH). Additional funding was from the Kenyon College Summer Science Scholars program. Funding sources had no role in the execution, writing, or decision to publish the study.
Conflict of interest
Authors have no conflicting interests to declare.
Data sharing
cDNA sequence is publicly available in the Genbank database with accession number MH457176. Other data that support the findings of this study are available from the corresponding author upon reasonable request.
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Present address: Penn State Health Milton S. Hershey Medical Center, Penn State College of Medicine, Hershey, PA USA.