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The cytochrome P450 (CYP) superfamily in cnidarians

Subjects

Abstract

The cytochrome P450 (CYP) superfamily is a diverse and important enzyme family, playing a central role in chemical defense and in synthesis and metabolism of major biological signaling molecules. The CYPomes of four cnidarian genomes (Hydra vulgaris, Acropora digitifera, Aurelia aurita, Nematostella vectensis) were annotated; phylogenetic analyses determined the evolutionary relationships amongst the sequences and with existing metazoan CYPs. 155 functional CYPs were identified and 90 fragments. Genes were from 24 new CYP families and several new subfamilies; genes were in 9 of the 12 established metazoan CYP clans. All species had large expansions of clan 2 diversity, with H. vulgaris having reduced diversity for both clan 3 and mitochondrial clan. We identified potential candidates for xenobiotic metabolism and steroidogenesis. That each genome contained multiple, novel CYP families may reflect the large evolutionary distance within the cnidarians, unique physiology in the cnidarian classes, and/or different ecology of the individual species.

Introduction

The cytochrome P450 superfamily

The cytochrome P450 (CYP) superfamily consists of a large group of hemeproteins that catalyze a wide range of reactions, playing important roles in several fundamental biological processes (e.g. steroid synthesis, fatty acid metabolism, chemical defense)1. CYPs primarily perform a monooxygenase function, adding polar hydroxyl groups to a substrate, making it more reactive and hydrophilic2. Each individual CYP has a specific suite of compounds that fit into its active site, often with a structure–activity relationship. Collectively, CYP enzymes interact with both endogenous (e.g. steroids and fatty acids) and exogenous (e.g. drugs, plant secondary metabolites, and pollutants) compounds with highly diverse chemical structures. Thus, the CYP superfamily plays a role in multiple, critical physiological processes. In vertebrates, the CYP11, CYP17, CYP19, CYP21 and CYP51 families catalyze steps in the synthesis of hormones, including sex steroids3. The CYP51 family, the only CYP family found in all domains of life, produces an intermediate, 4,4-dimethylcholesta-8(9),14,24-trien-3β-ol, in the cholesterol biosynthesis pathway4, the end product of which is an important component of the lipid bilayer and involved in cell signaling. Many of the enzymes in the CYP4 family play a role in the metabolism of omega fatty acids5, providing a source of adenosine triphosphate (ATP) for cells when carbohydrate stores are low. Certain proteins in the CYP1, CYP2, and CYP3 families have high substrate specificity for foreign compounds such as polycyclic aromatic hydrocarbons (PAHs) and drugs, modifying them as part of xenobiotic response and detoxification6,7.

CYP genes are named according to a standard set of nomenclature conventions based largely on sequence similarity8,9. CYPs with greater than 40% amino acid sequence identity belong to the same family (represented by a number) and those with greater than 55% sequence identity belong to the same subfamily (represented by a letter). Each CYP is assigned a gene number, typically based on order of discovery. As an example, CYP17A1 would be the first gene identified in the ‘A’ subfamily of the ‘CYP17′ family. A broader classification of CYPs into ‘clans’ has also been implemented, based on phylogenetic relationships among CYP families10. All of the CYP families that repeatedly cluster in the same phylogenetic clade are grouped into the same clan, which is usually given the name of the smallest number family present in that clade. For example, since CYP39, CYP7 and CYP8 sequences consistently form a single clade in phylogenetic analyses, all three families became part of clan 7.

The crucial nature of CYP proteins is emphasized by their presence in some capacity across all domains of life and they are thought to be present in all metazoan species11. The progression of genomic sequencing technologies has allowed the entire CYP gene complement (the CYPome) of many metazoan species to be identified, including those from major metazoan phyla. Studies have been completed on chordates7, model organisms such as mouse, fish, frog, and chicken, and fish such as Danio rerio (zebrafish)12 and Takifugu rubripes (fugu pufferfish)13. Other phyla that have been investigated in detail include the hemichordate Ciona intestinalis (sea squirt tunicate)14, echinoderm Stronglyocentrotus purpuratus (sea urchin)15, the arthropods Drosophila melanogaster (fruit fly)16 and Daphnia pulex (water flea crustacean)17, and the annelid Capitella teleta (marine worm)18. In many of these studies, full length and partial genes have been identified (as well as pseudogenes), along with estimations of intron–exon boundaries. In general, most vertebrate genomes tend to have between 50–100 CYP genes19, but the number of genes expected in other metazoan species is hard to predict as the diversity and evolutionary origins of individual CYP families is not well understood. For example, the genome of the annelid Capitella teleta contained 24 novel CYP families and 7 novel CYP subfamilies amongst its predicted total of 96 functional CYPs18. We can anticipate continued discovery of novel CYP genes where function is completely unknown as we sequence an increasingly broad diversity of metazoan genomes. While the number of novel CYPs varies across phyla (even the human genome contains the poorly understood “orphan” CYP20 enzyme)20, they are of great interest as identification of their function may provide important clues to the unique physiology and environmental stressors of different species, as well as the evolution of core physiological processes such as steroid biosynthesis.

Relatively little work has been done to identify cytochrome P450s in the species that comprise the cnidarian phylum, one of the most diverse and earliest-branching groups on the metazoan tree of life. One defensome study identified CYP sequences from the starlet sea anemone Nematostella vectensis, but the 82 genes were not named, in part due to their low similarity with known CYP genes21. With more recent genome sequencing in other cnidarians, notably the moon jellyfish Aurelia aurita22 and brown hydra Hydra vulgaris23 and stony coral Acropora digitfera24, we now have an opportunity to examine cnidarian CYPomes in detail.

The cnidarian phylum: evolutionary significance

There are more than 20,000 known cnidarian species, including many types of jellyfish, corals, anemones and other aquatic animals. Many of these species have become cost-effective models for research related to toxicology, regeneration and other biochemical systems25. Evidence from ribosomal DNA indicates that the common ancestor of the cnidarian phylum diverged from the rest of the metazoans approximately 600 million years ago26; although more recent molecular studies support an older divergence in the Neoproterozoic Era, around 600–800 million years ago27,28,29. This was before the split between protostomes (arthropods, annelids and mollusks) and deuterostomes (chordates, hemichordates, and echinoderms) that defines many of the species that have had their CYP content characterized (Fig. 1A). The lack of data on CYP genes from this area of the tree of life is a major gap in understanding CYP evolution in metazoans, and the functional role that CYPs may play in cnidarian physiology. There is extensive morphological, behavioural, developmental, and ecological diversity within the cnidaria and an understanding of CYP genes in the context of generation of biological signaling molecules and metabolism may be highly relevant to the diversity within this ancient lineage. The defining feature that unites the phylum is the presence of a specialized cell known as a cnidocyte, often referred to as the ‘stinging cell’. It produces a structure called a cnida (i.e. nematocyst) that contains toxins used as defense against predators and as a means of attack to capture prey25. Within the phylum, the three major lineages are the anthozoa, endocnidozoa and medusozoa; hydrozoans, scyphozoans and cubozoans are all in the medusozoa30. The anthozoan class is the most abundant in species and includes corals and anemones that reside on marine seafloors and act as habitats for other aquatic animals. The endocnidozoa consist of parasitic species. The medusozoan are the jellyfish, hydroids and siphonophores. Hydrozoans such as the brown hydra are small predatory animals that often live in salt and freshwater habitats, typically in large colonies. The scyphozoans (i.e. “true jellies”) and cubozoans (i.e. box jellyfish) play important roles in the pelagic food chain and ecology. Cnidarian life cycles can include swimming medusae and sessile polyp stages, asexual and/or sexual reproduction, free-living and parasitic stages, solitary or colonial groupings, and associations with photosynthetic dinoflagellates.

Figure 1
figure1

A simplified view of the cnidarian phylum in the tree of life. Branch lengths on the trees are arbitrary and meant only to visually display the relationship between the clades of species, not evolutionary distance between them. (A) The placement of the cnidarian phylum on the metazoan tree of life is highlighted. It diverged from the majority of metazoans, before the development of bilateral symmetry and the split between protostome and deuterostome development. (B) Cartoon of the relationships within the cnidarian phylum. The placement of A. aurita, H. vulgaris, A. digitifera and N. vectensis is illustrated. Adapted from25,30.

Complete genome assemblies had been published for several cnidarian species; we selected genomes from two of the three cnidarian classes: anthozoa (Nematostella vectensis, Acropora digitifera) and medusozoan (the hydrozoan Hydra vulgaris and the scyphozoan Aurelia aurita) (Fig. 1B)25; the Clytia genome has also recently been completed31. The hydrozoan H. vulgaris, commonly known as the brown hydra, has been studied as a model organism for regeneration and more recently, stem cell differentiation23. H. vulgaris is part of the Hydra vulgaris group, a group where species boundaries are uncertain and across which there is limited sequence diversity32. NCBI taxonomy considers H. magnipapillata33 and H. attenuata as heterotypic synonyms for H. vulgaris (NCBI:txid6087)34 and H. vulgaris strain 105 specifically denotes the hydra previously described as H. magnipapillata. We use H. vulgaris as the current taxonomy but H. magnipapillata was used with the genome release23. The anthozoan A. digitifera, or stony coral, is one of the main species that comprises the architecture of coral reefs, sustaining some of the most diverse marine ecosystems on the planet35. Another anthozoan, the starlet sea anemone N. vectensis, has become a model organism for gene knockout studies due to its quick developmental cycle36. Lastly, the schyphozoan moon jellyfish A. aurita has long been of interest to the scientific community due to its unique body plan and complex life cycle, as well as periodic ‘blooms’ of jellyfish that can have destructive effects on marine ecosystems37. A broad study of the defensome of N. vectensis was conducted by Goldstone21, including searching the genome for putative CYPs. A total of 82 potential CYP genes were identified, but at that time they were not grouped into existing families or subfamilies due to low amino acid sequence similarity with other known CYPs (< 40%)21. However, phylogenetic investigation revealed that the majority of these genes belonged in cytochrome P450 clans 2 and 3, which include CYPs from other organisms that metabolize both exogenous and endogenous compounds. These data suggest that detailed genomic and phylogenetic analyses of cnidarian CYPs presents an exciting opportunity to identify novel CYP families and subfamilies given the early divergence of the cnidaria from the bilateral metazoan and the ecological diversity among individual cnidarian species. The available genome sequences provide the means for a broad scope analysis of cytochrome P450 genes in the cnidarian phylum as a whole, as well as a comparison between three major classes. The goal of this study was thus to identify and characterize the cytochrome P450 superfamily in cnidarians, which could lead to the discovery of novel CYP families with unique functional properties, illuminate the ways that these species respond to environmental stressors, and to provide insight into the evolution of CYP functional diversity within the Metazoa.

Results

Genome-wide annotation of cytochrome P450 genes

For each cnidarian genome, well curated CYPs from other species (human, fruit fly, zebrafish, nematode worm, and annelid worm) were used in the basic local alignment search tool (BLAST) to identify regions of the genome that contained a likely CYP gene. Annotations were individually curated to locate, where possible, start and stop codons, appropriate signal sequences for intron–exon boundaries, an appropriate size of approximately 500 amino acids in translated protein sequence, and the presence and location of the key CYP gene motifs (I-helix, K-helix, meander coil and heme loop); expressed sequence tag (EST) support and a match to the Pfam CYP hidden markov model (HMM) were used to confirm identified CYP genes. The 82 CYP regions previously identified in N. vectensis were curated without further searching of the genome. In total, there were 19 cytochrome P450 genes found in the H. vulgaris genome, 14 in the A. digitifera coral species, 22 in the A. aurita moon jelly, and 44 in N. vectensis that met all criteria during curation (start and stop codon, translated to 500 aa, contained all of the CYP motifs). Many of the H. vulgaris gene predictions had strong EST support and all predicted complete genes in all species matched the entirety of the Pfam CYP model (HMM) with high confidence. Exon number was low in many of the predicted cnidarian CYP genes, with typically only 1–3 exons per gene; the only cnidarian CYPs with greater than 5 exons were found in the coral A. aurita.

There were several ‘partial’ CYPs genes identified in each species that were missing several hundred amino acid residues at the N-terminus or C-terminus of the protein (thus missing start and/or stop codons), but still contained all four of the key CYP motifs. There were 5 ‘partial’ CYPs in H. vulgaris, 10 in the A. digitifera coral, 15 in the A. aurita moon jelly, and 25 in N. vectensis. These partial genes contained enough genetic information that they are presumed functional, even though they are not completely resolved in the current genome assemblies available for each species. A list of all the ‘complete’ and ‘partial’ genes from each species, complete with their genomic location and length is available in Table S1. Each of these was assigned a formal name by the CYP Nomenclature Committee.

The length of each sequence and conservation of signature CYP motifs are summarized in Table 1 (H. vulgaris), Table 2 (A. digitifera), and Table 3 (A. aurita) for each of the newly identified complete and partial genes. The K-helix and heme loop motifs were the most highly conserved in all three cnidarian species; the glutamic acid and arginine residues in the K-helix were present in every gene and the only deviation in the heme loop was a fairly conservative G > A substitution in the A. aurita CYP3552G1 and a deletion in the CYP20 proteins we have observed in other metazoans (and noted in38). The I-helix and meander coil had significantly more variation between different CYP genes; the I-helix is degenerate in the CYP20 genes (a feature we and others38 have observed in metazoan CYP20s; Lemaire personal communication and data not shown) and while the phenylalanine, proline and arginine residues in the meander coil are highly conserved, the others vary considerably. This type of variation in the I-helix and meander coil is not uncommon in CYPs from other species and thus is not surprising for the cnidarians.

Table 1 The occurrence and position of conserved cytochrome P450 motifs in the H. vulgaris CYPome.
Table 2 The occurrence and position of conserved cytochrome P450 motifs in the A. digitifera CYPome.
Table 3 The occurrence and position of conserved cytochrome P450 motifs in the A. aurita CYPome.

As with all genome annotations of CYPs, multiple ‘fragments’ of CYPs were identified; the fragments varied in length, were missing one or more of the main CYP motifs, and it was unclear on whether they represented functional genes or pseudogenes (Table S2): 11 fragment genes in H. vulgaris, 34 in A. digitifera, 31 in A. aurita, and 14 in N. vectensis. Based on the complete and partial CYP gene sequences and setting aside the fragmentary gene sequences, the cnidarian genomes contain a minimum of 24 (H. vulgaris and A. digitifera), 37 (A. aurita), or 69 (N. vectensis) functional CYP genes and a total of 24 novel CYP families and 12 new subfamilies. Two of the new families are exclusive to H. vulgaris (CYP3353, CYP3354), another two are exclusive to A. digitifera (CYP3344, CYP3346), six are exclusive to N. vectensis (CYP377, CYP443, CYP3340, CYP3345, CYP3347, CYP3349), and four are exclusive to A. aurita (CYP3336-3337, CYP3341, CYP3351). In total, more than 85% of the complete or partial genes identified are from new CYP families and, other than the CYP20 genes and one CYP16 in N. vectensis, the rest are from new subfamilies within the CYP3, CYP4 and CYP46 clans.

Phylogenetic analysis of cnidarian cytochrome P450 sequences

The phylogenetic relationships between the cnidarian CYP genes are shown in Fig. 2. This maximum likelihood tree contains all of the complete and partial CYPs from each cnidarian species, but not the fragmentary genes. The phylogeny includes CYPs from humans, zebrafish and other vertebrates from eighteen vertebrate CYP families: CYP1-5, CYP7, CYP8, CYP11, CYP16, CYP17, CYP19-21, CYP24, CYP26, CYP27, CYP46 and CYP51. There are a total of 330 CYP sequences included in this tree. The vertebrate CYPs were clustered into their clans as expected and all clans had high bootstrap support (greater than 90%). Known species phylogeny was evident within the CYP gene families, both for the vertebrate species and those families where there were sequences from multiple cnidarian species. For example, N. vectensis and A. digitifera CYPs (the two anthozoan species) often clustered together, with representatives from each species in the CYP3094, CYP3339-CYP3340, CYP3342, and CYP3343-CYP3348 families clustered in the clan 2 and clan 3 clades. Likewise, H. vulgaris and A. aurita sequences always clustered together throughout the tree (CYP3351-3354 in clan 2, CYP4 and CYP20). In general, the cnidarian genes formed distinct clades within each clan (for example, the clan 2 H. vulgaris, clan 4 H. vulgaris and clan 3 A. aurita CYPs).

Figure 2
figure2

Maximum likelihood phylogenetic tree of cnidarian cytochrome P450 enzymes. The tree was generated with rapid bootstrapping and a gamma distribution with the JTT substitution matrix. Each CYP clan was assigned a different colour on the tree branches: clan 2 is purple, clan 3 is light green, clan 4 is blue, clan 7 is brown, clan 19 is red, clan 20 is dark green, clan 26 is orange, clan 46 is salmon, clan 51 is yellow, mitochondrial clan is turquoise. The five A. aurita CYPs that do not fit into established metazoan clans are light grey. The cnidarian CYPs are highlighted in dark grey on the perimeter of the tree. The different coloured asterisks indicate which cnidarian each CYP is from: H. vulgaris is brown, A. digitifera is black, A. aurita is yellow, N. vectensis is turquoise. The tree is rooted with the CYP51 family. Bootstrap values for each CYP clan, major CYP family divisions within each clan and major cnidarian clades are indicated on the tree. Bootstrap support for the placement of the branches that separate the individual clans was low (less than 50). Species acronyms are based on the family and species: Drer—zebrafish, Ggal—chicken, Hsap—human, Mmus—mouse, Rnor- rat, Xlae—frog, Trub—fugu pufferfish, Dnig—green pufferfish, Hvul—brown hydra, Adig—stony coral, Aaur—moon jellyfish, Nvec—starlet sea anemone.

Clan 2 contained the largest number of cnidarian sequences, most of which were in clades separate from any vertebrate sequences. Nonetheless, there were cnidarian sequences from the CYP3094 and CYP3349 family that clustered close to the CYP17 and CYP21 families and several cnidarian families (CYP3346, CYP3347, CYP3343, and CYP3348) that clustered with the CYP1 family. Vertebrate CYP27 and CYP24 families clustered with the cnidarian CYP3338, CYP377, and CYP375 families in the mitochondrial clan except for the CYP375D subfamily in N. vectensis, which is basal to the same clade. Phylogenetic analysis also had clear support for cnidarian CYP4, CYP20 and CYP46 family members. Interestingly, the phylogenetic results also supported N. vectensis having several genes related to CYP3N (CYP3662A1-3) and CYP3P (CYP3662B1) subfamilies, in addition to novel cnidarian CYP families (notably CYP3340) that clustered close to the vertebrate CYP5s in clan 3.

With the exception of five genes in A. aurita (CYP3336A1, CYP3336B1, CYP3336B2-1, CYP3336B2-2, and CYP3337A1), all of the cnidarian CYPs could be grouped into existing metazoan CYP clans. The proportion of each CYPome that fell into the major metazoan clans is shown in Fig. 3A. Clan 2 genes made up between 50 and 75% of each species’ CYPome, making it the most prevalent clan in each cnidarian genome. Interestingly, clan 3 was the second most prevalent (20–25%) for all of the cnidarians other than H. vulgaris, which lacked any complete or partial CYPs from this clan. While clan 4 CYPs represented a small portion of the N. vectensis and A. aurita CYPomes and were completely absent in A. digitifera, a relatively large proportion (25%) of the H. vulgaris CYPs fell in this clan. In total numbers this translates to only six clan 4 CYPs in H. vulgaris compared to two and one in N. vectensis and A. aurita, respectively. The mitochondrial clan CYPs were not highly prevalent in any of the cnidarian species (roughly 4–11% of the total CYPomes, except for H. vulgaris, where they were absent). Overall, when examining the presence/absence of the twelve metazoan CYP clans for each of the cnidarian species, the same clans were not found in all cnidarian genomes (Fig. 3B, Table S4). However, inclusion of fragmentary CYP genes finds clans 2, 3, 4 and 20 are present in all of four cnidarian species.

Figure 3
figure3

The distribution of cytochrome P450 genes among the metazoan CYP clans in four cnidarian species. (A) The proportion of each species’ CYPome that falls within the major metazoan clans (clan 2, clan 3, clan 4 and the mitochondrial clan). The number of CYP genes included in the analysis is indicated under each chart and includes all of the complete and partial CYPs from each species. Clan 16, clan 20 and clan 46 CYPs, as well as five A. aurita CYPs that did not fall discretely within any of the established metazoan CYP clans were designated as ‘Other’. (B) The presence or absence of each of the twelve metazoan CYP clans within each cnidarian species. Each column represents a different clan, and each row represents a different species. A filled black dot means that the clan was identified in the complete or partial genes, a white dot with a black outline means that the clan was identified in the fragmentary genes, and a white dot with a grey outline means that the clan was not found in the data. We have included CYP16 in Clan 16 because this clan designation has recently been determined by the nomenclature committee and other phylogenetic analyses support that CYP16 forms a separate clan61. In our phylogenetic analyses, the CYP16 genes clustered with Clan 26 genes (Fig. 2).

To better examine CYP family associations, phylogenetic trees were generated with only clan 2 sequences, including the CYP1, CYP2, CYP17 and CYP21 vertebrate families (Fig. 4; 121 sequences) or only clan 3 and 4 sequences, including the CYP3, CYP4 and CYP5 vertebrate families (Fig. 5; 61 sequences). The five A. aurita CYPs that did not place within an existing metazoan clan in Fig. 2, but were basal to the clan 3 and 4 CYPs, were included in the clan 3 and 4 tree. These subtrees generally had higher bootstrap support than the main tree and it was clear that the cnidarian CYPs formed distinct groups within the larger clan 2 clade; this pattern was observed both on the large tree containing all of the cnidarian CYPs (Fig. 2) and within the clan 2-specific tree (Fig. 4), with strong bootstrap support separating the major groups in both cases. Within clan 2, the CYP3343-CYP3348 families in N. vectensis and A. digitifera formed a sister clade to the CYP1 family of enzymes, while all of the H. vulgaris and A. aurita CYPs in this clan, as well as the CYP3094, CYP3349 and CYP3355 families from N. vectensis and A. digitifera, formed a large clade with the CYP17 and CYP21 vertebrate families, with varying degrees of relatedness. The phylogenetic tree of the clan 3 and clan 4 CYPs verified that the five uncategorized A. aurita CYPs were basal to those clans (Fig. 5). The cnidarian clan 3 CYPs formed a clade of exclusively cnidarian genes that were most closely related to CYP5 genes. Similarly, all of the cnidarian CYP4 genes formed a distinct group within the clan 4 clade most closely related to CYP4V genes, and each of the genes belonged to new CYP4 subfamilies.

Figure 4
figure4

Maximum-likelihood phylogenetic tree of cnidarian clan 2 cytochrome P450 enzymes. The tree was generated with rapid bootstrapping and a gamma distribution with the JTT substitution matrix. The CYP1 family and a sister cnidarian clade are salmon. The yellow branch identifies a large group of cnidarian CYPs and the vertebrate CYP17 and CYP21 families; this branch is further divided based on evolutionary distance to the vertebrate CYPs (blue is almost all CYPs that clustered directly with the vertebrate sequences, while the red and green groups both clustered outside of the vertebrate sequences). The cnidarian CYP names are highlighted in dark grey on the tree. The different coloured asterisks indicate which cnidarian each CYP is from: H. vulgaris is brown, A. digitifera is black, A. aurita is yellow, N. vectensis is turquoise. The tree is rooted with the CYP51 family. Bootstrap values for major CYP family divisions and major cnidarian clades are indicated on the tree. Species acronyms are based on the family and species: Drer—zebrafish, Ggal—chicken, Hsap—human, Mmus—mouse, Rnor- rat, Xlae—frog, Hvul—brown hydra, Adig—stony coral, Aaur—moon jellyfish, Nvec—starlet sea anemone.

Figure 5
figure5

Maximum-likelihood phylogenetic tree of cnidarian clan 3 and clan 4 cytochrome P450 enzymes. The tree was generated with rapid bootstrapping and a gamma distribution with the JTT substitution matrix. The Clan 3 CYPs are light green, the Clan 4 CYPs are dark blue, and the CYPs that do not fall within a clan are grey. The cnidarian CYP names are highlighted in dark grey on the tree. The different coloured asterisks indicate which cnidarian each CYP is from: H. vulgaris is brown, A. digitifera is black, A. aurita is yellow, N. vectensis is turquoise. The tree is rooted with the CYP11 family. Bootstrap values for each CYP clan, major CYP family divisions within each clan and major cnidarian clades are indicated on the tree. Species acronyms are based on the family and species: Drer—zebrafish, Hsap—human, Mmus—mouse, Rnor- rat, Xlae—frog, Hvul—brown hydra, Adig—stony coral, Aaur—moon jellyfish, Nvec—starlet sea anemone.

Each of the phylogenetic trees included annotated CYPs from vertebrate species. Inclusion of invertebrate CYPs from D. melanogaster, C. elegans, and C. teleta interfered negatively with tree construction, often resulting in low bootstrap support (< 50%). This has been reported in other studies using both vertebrate and invertebrate sequences16,18. Even with the vertebrate sequences, the deeper branches that separate the clans in Fig. 3 had some bootstraps under 50% (not shown on the tree), likely due to the evolutionary distance that separates the species between the various phyla. However, the relationship between the clans on this tree remains consistent with trends that are commonly seen in maximum-likelihood CYP analysis12,13,21 and bootstrap support for the individual clans remained high. The tree was rooted with the CYP51 family because CYP51 is the only CYP family found in all domains of life (including bacteria and viruses), and thus is thought to be the first eukaryotic CYP44,10; CYP51 genes are commonly used to root trees in CYP phylogenetic analyses19. The same root was chosen for the clan 2 phylogeny and the mitochondrial clan CYP11 family was used to root the clan 3 and 4 phylogeny. Subtree roots were chosen from clans that typically form basal clades to the main clans being analyzed in those subtrees12,13.

Discussion

Cnidarian CYPomes

The genomic analysis of H. vulgaris, N. vectensis, A. digitifera and A. aurita demonstrated that cnidarian CYPomes are highly diverse, with 24 novel CYP families and 12 novel subfamilies involving more than 85% of the predicted cnidarian CYP genes. This means that a majority of cytochrome P450 genes in cnidarians are less than 40% similar to all other documented genes in this superfamily, a testament to more than 500 million years of natural selection and diversification26. There are other cnidarian gene families which have proven to be unique from their metazoan counterparts. For example, innexin transmembrane proteins identified in H. vulgaris were only 25% identical to similar genes in protostomes39. Similarly, while there are many identified precursors of neuropeptide signaling genes in N. vectensis (such as RPamides, RWamides, and VRamides), none of them are confirmed orthologs of bilaterian neuropeptides40. However, there is not always a significant difference between cnidarian sequences and other studied metazoans. The Wnt signaling protein family is largely conserved between cnidarians and vertebrates, as most major subfamilies are present in both phyla41,42. Additionally, an examination of the SOX transcription factor gene family in cnidarians identified clear bilaterian orthologs along with expected expression patterns43. This makes it clear that certain gene families arose in an early metazoan ancestor and remained largely unchanged in cnidarians, while others such as the cytochrome P450 superfamily arose early in the history of metazoans but were subject to significant change in this phylum. Using sequence similarity to known genes does have its challenges, particularly when there is bias in the taxonomic sampling across the tree of life. Much of the known CYP genes are from eukaryotes and of the metazoan sequences, vertebrates and insect sequences dominate (see the Cytochrome P450 Homepage; https://drnelson.uthsc.edu/CytochromeP450.html). Thus, it will be highly interesting to reassess the unique cnidarian genes and determine which are the result of duplications within the cnidarian lineage and which have non-vertebrate orthologs. Much better taxonomic sampling, both within and near the cnidarians, would be helpful to address this question.

There is clear diversity in the cytochrome P450 complement across the cnidarians as a phylum. Figure 3 demonstrates that, when considering gene number, proportion of CYPs belonging to particular clans, and the presence/absence of different CYP clans, none of the four species considered were exactly the same. Differences between the N. vectensis and H. vulgaris genome have been well documented, since they were the first two cnidarian species to be fully sequenced; both in terms of general observations such as genome size, but also in terms of other specific genes such as the 301 family epitheliopeptides and the SWT domain of receptors and secreted proteins44. Publication of the A. digitifera genome additionally identified that there are marked differences in the repertoire of TIR-domain-containing proteins between A. digitifera, N. vectensis, and H. vulgaris24. The four cnidarian species analyzed here differ in total CYP number and in the families and clans of CYPs that are present in their genomes. There are certain families that were exclusive to a particular species (Table S3); based on the phylogenetic history of the phylum25,30 (Fig. 1B) it is possible to infer when these families arose relative to the speciation events that formed the different classes and species. Table S3 identifies the CYP families by species and indicates likely gene gain or loss by species or class. In general, N. vectensis has a much larger CYP gene complement than the other cnidarians and that is largely based on gene gains, even in CYP families shared with A. digitifera (e.g. 17 CYP3094 genes versus 5 in A.digitifera; 7 CYP3342 genes versus 1 in A. digitifera). Gene expansions are common among CYP families in other species, including those as diverse as mouse, sea urchin, and mosquito. These expansions are often in CYP families involved in responding to the chemical environment, although in many cases little is known about the enzyme function. Gene expansions have been previously identified in Anthozoans22; what novel functions are afforded N. vectensis from the CYP gene expansions are not clear.

Fourteen of the new families (CYP377, CYP443, CYP3094, CYP3339, CYP3340, CYP3342-3349 and CYP3355) were exclusive to the anthozoan class, meaning these likely arose after the anthozoans diverged from the remainder of the cnidarians. Of these families, CYP3094, CYP3339, CYP3342, CYP3343, CYP3348 and CYP3355 are found in both A. digitifera and N. vectensis, indicating that these families likely arose after the anthozoan split from the rest of the cnidarians, but before the split between the two species within this class. CYP3344, CYP3346, and CYP3348 are exclusive to A. digitifera while CYP377, CYP3340, CYP3345, CYP3347, and CYP3349 are exclusive to N. vectensis, which means these families likely arose separately after the split of the lineages including these species. CYP443 was exclusive to N. vectensis in this gene set, but CYP443 genes have been found in A digitifera, A. palmate, A. millepora, Aiptasia pallida and Anemonia viridis (D. Nelson, unpublished data), suggesting this is gene family is not exclusive. CYP443 are in Clan74 and are found in only a few animal species. Five CYP families (CYP334, CYP3336-3338 and CYP3351) are exclusive to the scyphozoan species and just two (CYP3353 and CYP3354) are exclusive to the hydrozoan species. The CYP3352 family is present in both H. vulgaris and A. aurita, which means it likely arose after the anthozoan split, but before the split between hydrozoan and scyphozoans. The presence of multiple species-exclusive CYP families is likely the result of exposure to different selective pressures and environments over time. Even the two anthozoan species, which are presumed to be the most similar to each other based on phylogenetics, diverged roughly 520–490 million years ago24. That means there was a significant period of time (> 500 million years) when these cnidarian lineages were exposed to different environments, had access to different resources, and were differentially exposed to other factors that would influence CYP evolution.

Cnidarian CYP Clans

The CYP clan framework was implemented as a means to describe the recurring deep branching clusters observed in metazoan CYP phylogenies9. The clans provide a way to describe and characterize the complexity of CYP evolution between species. Multiple phylogenetic analyses have established certain relationships between the metazoan CYP clans; for example, clan 3 and clan 4 consistently form sister clades in metazoan phylogenies17,19,21. These same patterns are observed in the trees generated for this study, although the bootstrap support is not high for this grouping in this phylogeny (Fig. 2). The presence and absence of each clan has been examined in multiple phyla, establishing expectations for which clans are present in different types of species. Almost all metazoans, excluding certain early-branching phyla such as ctenophores, have CYPs from clans 2, 3, 4, and the mitochondrial clan19. When fragmentary genes are considered, this is true for all of the cnidarian species analyzed (Fig. 3B). Large clan losses have been documented in certain phyla as well, particularly in nematodes and arthropods19. Our analysis indicates that clans 7 and 51 were lost in the cnidarian phylum as a whole; CYP19 is not present in any cnidarian genome (Fig. 3B). Examining the phylogenetic relationships between the cnidarian CYPs and clans provides conservative hypotheses about what types of CYPs are present in these species, based on the evolutionary distance between the sequences. Clan 2 genes were especially abundant in the cnidarian CYPomes and are discussed in detail, as is the particularly interesting loss of clan 51.

Clan 2

In general, the clan 2 genes are the most prevalent CYPs in all four cnidarians (approximately 50% of the N. vectensis and A. aurita CYPomes and approximately 75% of the A. digitifera and H. vulgaris CYPomes), which is also the case in humans7, zebrafish12, the tunicate Ciona intestinalis14, the marine annelid Capitella teleta18, and the echinoderm Stronglyocentrotus purpuratus15. The clan 2 phylogenetic tree (Fig. 4) elaborates on the relationships seen in the larger phylogeny (Fig. 2), with high bootstrap support. None of the cnidarian genes clustered with the CYP2 family, which is prominent in vertebrates and includes enzymes that catalyze arachidonate and drug metabolism. In contrast, CYP1 genes and other CYP families (sometimes referred to as “CYP1-like”) have frequently been found to closely cluster with CYP1s in other species, such as tunicates14, annelids18, and the sea urchin15. In cnidarians, the CYP3343-CYP3348 families from N. vectensis and A. digitifera, formed a large clade with the CYP1 family, making these cnidarian genes strong candidates for xenobiotic metabolism. The CYP1 family is critical for the metabolism of planar, halogenated compounds such as polycyclic aromatic hydrocarbons in vertebrates6,7 and there is evidence that cnidarians (N. vectensis in particular) respond to PAHs and weathered oil through increased expression of certain CYPs as well as antioxidant enzymes such as superoxide dismutases and catalases45,46 (Berger and Tarrant personal communication).

A large group of cnidarian clan 2 CYPs form a clade with the CYP17 and CYP21 families, which are directly linked to steroidogenesis in vertebrates. The CYP17A1 gene in humans, also known as steroid 17α-monooxygenase/17,20-lyase, oxidizes pregnenolone or progesterone, which is one of the first steps in androgen or corticoid synthesis following cholesterol side-chain cleavage47. The CYP21A1 gene, or steroid 21-hydroxylase, catalyzes the hydroxylation of progesterone and 17α-hydroxyprogesterone, one of the intermediate steps in the synthesis of the stress hormone cortisol48. The CYP3094 and CYP3349 families in N. vectensis and A. digitifera form a clade immediately basal to the CYP17/21 genes, while the CYP3355 families were clearly outside of this clade (Fig. 4). There are a total of sixty-seven cnidarian enzymes in this large group of CYPs (25 N. vectensis, 6 A. digitifera, 17 H. vulgaris and 19 Aurelia), with particularly large expansions of the CYP3352 family in H. vulgaris and A. aurita and the CYP3094 family in N. vectensis and A. digitifera. Most species typically have a fairly low copy number of steroidogenic CYPs (for example, humans have only one CYP17A1 gene7 and zebrafish have only two12), which means it is unlikely that all of these genes are steroidogenic. Similarly, the presence of multiple clan 46 genes in N. vectensis is surprising. The CYP46 family, or cholesterol 24-hydroxylase, modifies cholesterol so that it can pass through the blood–brain barrier in humans and be metabolized in the liver49. In vertebrates these genes are usually present in low copy number, with only one in humans7 and two in zebrafish12. CYP46 copy number is likewise low in the scallop Chlamys farreri (2)50, the polychaete C. teleta (1)18, and the ctenophore Mnemiopsis leidyi19 but was much higher in four species of Brachionus rotifers (7–8 per species51). There are seven CYP46 genes in N. vectensis. Although the N. vectensis nervous system lacks a brain-like centre or core, the molecular function of these CYPs is presumed to be similar to their vertebrate homologs based on high sequence similarity52.

The capacity to synthesize estrogen de novo by cnidarians has been demonstrated in the anthozoans Scleractinia53 and Montipora54. In vertebrates, select CYP families (CYP11, CYP17, CYP19, CYP21, CYP51) and hydroxysteroid-dehydrogenase enzymes play important roles in steroidogenesis, including estrogen production55. However, there were few cnidarian CYPs that qualify as candidate homologs of vertebrate steroid synthesis genes. No cnidarian CYP gene clustered with the CYP19 or CYP51 families and the cnidarian CYPs in the mitochondrial clan clearly do not cluster with the CYP11 family (Fig. 2). Thus, if CYPs play a major role in de novo estrogen production in cnidarians, it is likely that the CYP family (or families) involved are phylogenetically distinct from the vertebrate genes, and pinpointing the exact genes will be challenging. The best candidates in our results are the CYPs in phylogenetic proximity to the steroidogenic CYP17 and CYP21 vertebrate families (Fig. 2), such as CYP3094K1, CYP3094K2, and CYP3094A1 from the anthozoans N. vectensis and A. digitifera.

Clan 51

Clan 51, which consists entirely of the CYP51 family, was not present in any of the cnidarian genomes analyzed in this study, even when potential pseudogenes or gene fragments were considered. The lack of CYP51 genes is interesting as this family encodes lanosterol 14 α-demethylase, which catalyzes an essential step in the biosynthesis of cholesterol56. This family has been found in molluscs, annelids, and sponges in addition to vertebrates, but is absent in insects, crustaceans, and nematodes19, and some tunicates57. The absence of this family from the cnidarian species studied here implies that these species lack de novo cholesterol synthesis and would need to receive this important signaling molecule from their environment and diet. Studies on the evolution of the cholesterol biosynthesis genes found losses in Cnidaria58. This is in line with research that indicated cholesterol as the most prominent sterol (50–63%) in lipid samples of cnidarians as a result of their generally carnivorous diet59. There is varying data regarding de novo cholesterol biosynthesis in cnidaria57, as for example, some, but not all, anthozoa tested in one study exhibited de novo sterol synthesis60. Thus obligate dietary cholesterol may be a character that varies within cnidaria, and indeed even within anthozoa.

Hydra vulgaris

The CYPome of H. vulgaris is of special interest due to several unique differences from the CYPomes of other species. There were 24 complete CYP genes predicted in H. vulgaris and only 11 fragments that may or may not be functional. This is smaller than most reported metazoan CYPome; to date, the sponge Amphimedon queenslandica with 35 genes19 and the tomato russet mite Aculops lycopersici with 23 genes61 have the smallest CYPomes. The results for H. vulgaris are a large departure from the 69 predicted CYPs in N. vectensis, which is comparable to most vertebrate CYPomes (usually around 50–100 genes)19 and other species such as the crustacean Daphnia pulex (75 CYPs)17 and the sea urchin Stronglyocentrotus purpuratus (120 CYPs)15. While there were only 24 CYPs predicted in A. digitifera, there were 34 fragments, which means it is possible that this coral CYPome is considerably larger.

Certain CYP families (CYP375, CYP3350) are present in the anthozoan and scyphozoan cnidarians, but absent in the hydrozoan H. vulgaris. The phylogenetic history of the cnidaria (Fig. 1B) suggests that any gene families present in anthozoans and scyphozoans arose in the ancestral cnidarian and would be present in hydrozoans as well unless lost. Thus, clan 3 genes were identified in all of the cnidarian species except for H. vulgaris, yet clan 3 CYPs are believed to have been present in very early animals, before the origins of cnidarians19. As indicated in Fig. 3B, a single gene fragment in H. vulgaris had high sequence similarity to CYP3 genes from other species, but it was missing the critical CYP heme loop motif (Table S2) and may represent a pseudogene. Regardless, it is clear that clan 3 genes have undergone a significant reduction in H. vulgaris when compared to the other cnidarians (Fig. 3A). A similar reduction in gene count is observed in the mitochondrial CYP clan in H. vulgaris (Fig. 3B).

All of this evidence suggests that extensive loss of CYP genes and clans has occurred in H. vulgaris, more so than the other cnidarian species analyzed, in agreement with observations by other researchers that considerable gene loss has occurred in the Hydra genome as a whole. For example, while N. vectensis has roughly 140 homeobox genes from nearly 60 gene families, H. vulgaris only has about 50 homeobox genes from 30 gene families (no such reduction has been observed in A. digitifera)62. The genomic origin of the Hox gene cluster is thought to be a close neighbour to the original cytochrome P450 locus that expanded to form the large CYP superfamily, which provides further support for the smaller Hydra CYPome19. More than half of the H. vulgaris genome is composed of repetitive elements (including transposable elements) and estimates of protein-coding gene number are significantly lower in this species23. There is no clear explanation for this reduction in genome size and loss of multiple gene families in H. vulgaris, although it is correlated with lack of a larval stage in the H. vulgaris life cycle. Given the reduced H. vulgaris CYPome, determining the function of the novel H. vulgaris CYPs is of particular interest.

Annotation and phylogenetic analysis of cytochrome P450 genes

Precise gene annotation and phylogenetic analysis can be difficult when studying species that are distantly related to those with well-studied and defined CYPomes. The CYPs used to search the cnidarian genomes were well curated genes from humans, D. rerio, D. melanogaster, C. elegans, and C. teleta. As Tables 1, 2 and 3 indicate, all four significant P450 motifs are generally well conserved in the cnidarian CYPs. The I-helix motif ([AG]G-x-[DE]T[TS]) has been shown to play a role in proton delivery for the reactions that CYPs catalyze, while the K-helix (E-x-x-R) and meander coil (FDPER) are thought to stabilize the core structure of the protein through salt bridge interactions63. The heme loop (F-x-x-G-x-R-x-C-x-G) is arguably the most important of the four because it facilitates association with the heme cofactor in the active site64. Other than a few known exceptions (for example, the CYP20 family is missing the I-helix motif and contain a deletion in the heme loop (K. Pankov, personal observation)—both observed in our cnidarian data), the large majority of metazoan cytochrome P450 enzymes maintained the presence of these four motifs and their relative position in CYP proteins was conserved. Of the predicted cnidarian CYPs, there were only a few predicted amino acid substitutions in the I-helix or meander coil and perfect matches to the K-helix and heme loop motifs in all cases, suggesting accurate prediction of gene models in these cnidarian genomes. However, multiple partial genes and gene fragments were identified in each annotated genome, which could be the result of evolutionary processes or artifacts of genome sequencing and assembly (albeit 90% of the H. vulgaris and A. digitifera genomes are estimated to be present in the current assemblies)23,24. By our definition, partial sequences had sufficient length to identify all conserved CYP motifs, with a strong match to the P450 HMM, and EST coverage when applicable; increasing our confidence that the partial genes encode functional CYP genes but that their sequences include genome assembly gaps. For example, certain partial CYPs on Contig36189 for H. vulgaris and Contig NW_015441134.1 for A. digitifera have sequencing gaps directly upstream of the predicted genes. The predicted fragmentary genes are more problematic—additional research will be needed to determine if they reflect real pseudogenes or genome sequencing artifacts. However, pseudogenes are common in the CYP superfamily, since much of the diversity of cytochrome P450s arose from multiple tandem gene duplications65, and there is clear evidence for tandem CYP gene duplication in all of the cnidarian genomes (Table S1). There were 13 potential pseudogenes in the annelid C. teleta CYPome18 and 17 in the vertebrate Fugu CYPome13, comparable to the fragmentary genes found in the cnidarian genomes: 11 gene fragments in H. vulgaris, 34 in A. digitifera, 31 in A. aurita, and 14 in N. vectensis.

Conclusion

Gene annotation has made it clear that there is significant diversity between cnidarian CYPomes, even when those species belong in the same class. Over 500 million years of evolutionary history has expanded cnidarian CYPomes in some clans (especially clan 2) and resulted in extensive loss in others (clan 3 and mitochondrial clan CYPs). Certain cnidarians have a relatively large and diverse set of CYPs (the starlet sea anemone and the moon jellyfish), while others have a smaller, less diverse CYP complement (the stony coral and the brown hydra). Overall, cnidarian CYPs are found in nine of the twelve metazoan CYP clans; clan 16 is the most recent61. Yet, our analysis identified 24 novel cnidarian CYP families. This presents exciting opportunities for discovery of new functional capabilities of the cytochrome P450 superfamily in the context of metazoan and cnidarian evolution. This study presents several cnidarian candidates for genes with detoxification roles (CYP3343-3348 in the anemone and coral) and many more from all four cnidarians that could be involved in steroidogenesis66,67. All of the predicted functional cytochrome P450s in H. vulgaris, A. digitifera, N. vectensis, and A. aurita have been identified with confidence. Functional assays and in silico methods such as structural modeling and substrate docking may provide additional clues to the role of these cnidarian enzymes.

Methods

Genome-wide annotation of cytochrome P450 genes

The first versions of the genome assemblies for each species (H. vulgaris, A. digitifera, A. aurita) were searched for cytochrome P450 genes. The Basic Local Alignment Search Tool (v2.2.31)68 was used to identify local alignments between the cnidarian genomes and a query that consisted of all annotated CYPs in humans and zebrafish (vertebrate) and select CYPs in D. melanogaster (arthropod), C. elegans (nematode), and C. teleta (annelid) in a TBLASTN search (protein query against a genome nucleotide). Though previous efforts had been successful with just vertebrate queries18, a large variety of sequences from across metazoans were included to maximize CYP gene identification. Only those BLAST high scoring pairs with expectation values of 1.0 × 10–11 or smaller were considered significant.

The JBrowse genome viewer (v1.12.1)69 was used to manually annotate the significant regions of each genome from the BLAST results, identifying start (ATG) and stop (TGA/TAA/TAG) codons, plus introns, exons, and splice site signals (GT/AG) at intron–exon boundaries. Expressed sequence tag (EST) data sets publicly available for both H. vulgaris and A. aurita were aligned to the respective genomes with BLAT (BLAST-like alignment tool)70 as an aid to identification of genes, intron–exon boundaries, and confirmation of gene expression. The H. vulgaris EST data set consisted of approximately 18,000 individual reads23 while the A. aurita EST data set contained only 77 reads37.

Potential CYPs in each cnidarian species were identified, considered full length at ~ 500 amino acid residues, and were matched to the well-curated cytochrome P450 HMM in the Pfam protein family database71 to confirm identity. The ScanProsite tool72 was used to verify the presence of four largely conserved CYP motifs: the I-helix, K-helix, meander coil and heme loop. Pfam and Prosite scans included the 82 N. vectensis CYPs previously identified but not named21. Each putative CYP was classified as complete (proper length with start and stop codon, all motifs present, and match to the HMM) or partial (presence of at least the entire ~ 120 amino acid region that contains all motifs, but clearly less than full length). Any potential CYP that was missing at least one of the Prosite motifs was considered a gene fragment. The resulting complete cnidarian CYPs were used as queries for another BLAST search of each species’ genome to ensure that all paralogs were identified.

Phylogenetic analysis of cnidarian cytochrome P450 sequences

All of the complete and partial CYPs were included in phylogenetic analyses, plus the previously predicted CYP protein sequences for N. vectensis21, with all predicted CYP proteins assigned a formal name by the CYP Nomenclature Committee. Clustal Omega (v1.2.4)73 was used to generate a global multiple sequence alignment of all H. vulgaris, A. digitifera, N. vectensis and A. aurita sequences plus a variety of vertebrate CYPs, including all major families from humans and Danio rerio, and select families from Mus musculus, Xenopus laevis, Rattus norvegicus, Gallus gallus, Takifugu rubripes, and Dichotomyctere nigroviridis (over 300 sequences in total). Mesquite (v3.10)74 was utilized to remove poorly aligned regions of uncertain homology, especially at the termini of the protein sequences where significant variation is typically observed. The final trimmed alignment was used as input for the Randomized Axelerated Maximum Likelihood Program (RAxML v8.2.9)75, with the rapid generation algorithm (-x), a gamma distribution for among-site rate variation, the JTT substitution matrix with empirical amino acid frequencies, and 100 bootstrap replicates for assessment of phylogenetic confidence. The final maximum likelihood phylogenetic tree was visualized with Figtree (v1.4.3)76 and rooted using the CYP51 family of enzymes. Clan-specific multiple sequence alignments and phylogenetic trees were generated using the same process, restricted to include only sequences that clustered with a particular clan in the global phylogeny. The clan 2 tree was rooted with CYP51, while the clan 3 and 4 trees were rooted with the CYP11 family.

Data availability

No new sequence data were generated, previously published accessions are included in the manuscript.

References

  1. 1.

    Danielson, P. B. The cytochrome P450 superfamily: Biochemistry, evolution and drug metabolism in humans. Curr. Drug Metab. 3, 561–597 (2002).

    CAS  PubMed  Article  Google Scholar 

  2. 2.

    Hill, H. A. O., Roder, A. & Williams, R. J. P. Cytochrome P-450: Suggestions as to the structure and mechanism of action. Nature 57, 69–72 (1970).

    CAS  Google Scholar 

  3. 3.

    Zhang, L. H., Rodriguez, H., Ohno, S. & Miller, W. L. Serine phosphorylation of human P450c17 increases 17,20-lyase activity: Implications for adrenarche and the polycystic ovary syndrome. Proc. Natl. Acad. Sci. USA 92, 10619–10623 (1995).

    ADS  CAS  PubMed  Article  Google Scholar 

  4. 4.

    Lepesheva, G. I. & Waterman, M. R. Sterol 14α-Demethylase Cytochrome P450 (CYP51), a P450 in all biological kingdoms. Biochim. Biophys. Acta 1770, 467–477 (2007).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  5. 5.

    Arnold, C., Konkel, A., Fischer, R. & Schunck, W. H. Cytochrome P450-dependent metabolism of omega-6 and omega-3 long-chain polyunsaturated fatty acids. Pharmacol. Rep. 62, 536–547 (2010).

    CAS  PubMed  Article  Google Scholar 

  6. 6.

    Lewis, D. F. Human cytochromes P450 associated with the phase 1 metabolism of drugs and other xenobiotics: A compilation of substrates and inhibitors of the CYP1, CYP2 and CYP3 families. Curr. Med. Chem. 10, 1955–1972 (2003).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  7. 7.

    Lewis, D. F. 57 varieties: The human cytochromes P450. Pharmacogenomics 5, 305–318 (2004).

    CAS  PubMed  Article  Google Scholar 

  8. 8.

    Nelson, D. R. et al. P450 superfamily: Update on new sequences, gene mapping, accession numbers and nomenclature. Pharmacogenet 6, 1–42 (1996).

    CAS  Article  Google Scholar 

  9. 9.

    Nelson, D. R. Metazoan cytochrome P450 evolution. Comp. Biochem. Physiol. C Pharmacol. Toxicol. Endocrinol. 121, 15–22 (1998).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  10. 10.

    Nelson, D. R. Cytochrome P450 and the individuality of species. Arch. Biochem. Biophys. 369, 1–10 (1999).

    CAS  PubMed  Article  Google Scholar 

  11. 11.

    Nelson, D. R. Progress in tracing the evolutionary paths of cytochrome p450. Biochem. Biophys. Acta 1814, 14–18 (2011).

    CAS  PubMed  Google Scholar 

  12. 12.

    Goldstone, J. V. et al. Identification and developmental expression of the full complement of cytochrome P450 genes in zebrafish. BMC Genomics 11, 643. https://doi.org/10.1186/1471-2164-11-643 (2010).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  13. 13.

    Nelson, D. R. Comparison of P450s from human and fugu: 420 million years of vertebrate P450 evolution. Arch. Biochem. Biophys. 409, 18–24 (2003).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  14. 14.

    Goldstone, J. V. et al. Cytochrome P450 1 genes in early deuterostomes (tunicates and sea urchins) and vertebrates (chicken and frog): origin and diversification of the CYP1 gene family. Mol. Biol. Evol. 24, 2619–2631 (2007).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  15. 15.

    Goldstone, J. V. et al. The chemical defensome: environmental sensing and response genes in the Stronglyocentrotus purpuratus genome. Dev. Biol. 300, 366–384 (2006).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  16. 16.

    Tijet, N., Helvig, C. & Feyereisen, R. The cytochrome P450 gene superfamily in Drosophila melanogaster: annotation, intron-exon organization and phylogeny. Gene 262, 189–198 (2001).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  17. 17.

    Baldwin, W. S., Marko, P. B. & Nelson, D. R. The cytochrome P450 (CYP) gene superfamily in Daphnia pulex. BMC Genomics 10, 169. https://doi.org/10.1186/1471-2164-10-169 (2009).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  18. 18.

    Dejong, C. A. & Wilson, J. Y. The cytochrome P450 superfamily complement (CYPome) in the annelid Capitella teleta. PLoS ONE 9, e107728. https://doi.org/10.1371/journal.pone.0107728 (2014).

    ADS  CAS  Article  PubMed  PubMed Central  Google Scholar 

  19. 19.

    Nelson, D. R., Goldstone, J. V. & Stegeman, J. J. The cytochrome P450 genesis locus: The origin and evolution of animal cytochrome P450s. Philos. Trans. R. Soc. B Biol. Sci. 368, 20120474. https://doi.org/10.1098/rstb.2012.0474 (2013).

    CAS  Article  Google Scholar 

  20. 20.

    Guengerich, F. P. & Cheng, Q. Orphans in the human cytochrome p450 superfamily: Approaches to discovering functions and relevance in pharmacology. Pharmacol. Rev. 63, 684–699 (2011).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  21. 21.

    Goldstone, J. V. Environmental sensing and response genes in cnidaria: The chemical defensome in the sea anemone Nematostella vectensis. Cell Biol Toxicol 24, 483–502 (2008).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  22. 22.

    Gold, D. A. et al. The genome of the jellyfish Aurelia and the evolution of animal complexity. Nat. Ecol. Evolut. 3, 96–104 (2019).

    Article  Google Scholar 

  23. 23.

    Chapman, J. A. et al. The dynamic genome of Hydra. Nature 464, 592–596 (2010).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  24. 24.

    Shinzato, C. et al. Using the Acropora digitifera genome to understand coral responses to environmental change. Nature 476, 320–323 (2011).

    ADS  CAS  PubMed  Article  Google Scholar 

  25. 25.

    Brusca, R. C., Wendy, M. & Shuster, S. M. Invertebrates 3rd edn. (Oxford University Press, 2016).

    Google Scholar 

  26. 26.

    Sullivan, J. C., Retizel, A. M. & Finnerty, J. R. A high percentage of introns in human genes were present early in animal evolution: Evidence from the basal metazoan Nematostella vectensis. Genome Inform. 17, 219–229 (2006).

    CAS  PubMed  Google Scholar 

  27. 27.

    Dohrmann, M. & Wörheide, G. Dating early animal evolution using phylogenomic data. Sci. Rep. 7, 3599 (2017).

    ADS  PubMed  PubMed Central  Article  CAS  Google Scholar 

  28. 28.

    Gold, D. A. Life in changing fluids: A critical appraisal of swimming animals before the Cambrian. Integr. Comp. Biol. 58, 677–687 (2018).

    PubMed  Article  Google Scholar 

  29. 29.

    Park, E. et al. Estimation of divergence times in cnidarian evolution based on mitochondrial protein-coding genes and the fossil record. Mol. Phylogenet. Evol. 62, 329–345 (2012).

    PubMed  Article  Google Scholar 

  30. 30.

    Kayal, E. et al. Phylogenomics provides a robust topology of the major cnidarian lineages and insights on the origins of key organismal traits. BMC Evol. Biol. 18, 68 (2018).

    PubMed Central  Article  CAS  Google Scholar 

  31. 31.

    Leclère, L. et al. The genome of the jellyfish Clytia hemisphaeric and the evolution of the cnidarian life-cycle. Nat. Ecol. Evol. 3, 801–810 (2019).

    PubMed  Article  PubMed Central  Google Scholar 

  32. 32.

    Martínez, D. E. et al. Phylogeny and biogeography of Hydra (Cnidaria: Hydridae) using mitochondrial and nuclear DNA sequences. Mol. Phylogenet. Evol. 57, 403–410 (2010).

    PubMed  Article  CAS  Google Scholar 

  33. 33.

    Itô, T. A new fresh-water polyp, Hydra magnipapillata, n. sp. from Japan. Sci. Rep. 18, 6–10 (1947).

    Google Scholar 

  34. 34.

    Pallas, P. S. Elenchus Zoophytorum. Apud Petrum van Cleef, Hagae-Comitum (1766).

  35. 35.

    Hinrichs, S., Patten, N. L., Feng, M., Strickland, D. & Waite, A. M. Which environmental factors predict seasonal variation in the coral health of Acropora digitifera and Acropora spicifera at Ningaloo Reef?. PLoS ONE 8, e60830. https://doi.org/10.1371/journal.pone.0060830 (2013).

    ADS  CAS  Article  PubMed  PubMed Central  Google Scholar 

  36. 36.

    Genikhovich, G. & Technau, U. The starlet sea anemone Nematostella vectensis: An anthozoan model organism for studies in comparative genomics and functional evolutionary developmental biology. Cold Spring Harb. Protoc. 2009, pdb.emo129. https://doi.org/10.1101/pdb.emo129 (2009).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  37. 37.

    Brekhman, V., Malik, A., Haas, B., Sher, N. & Lotan, T. Transcriptome profiling of the dynamic life cycle of the scyphozoan jellyfish Aurelia aurita. BMC Genomics 16, 74. https://doi.org/10.1186/s12864-015-1320-z (2015).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  38. 38.

    Lemaire, B. et al. Cytochrome P450 20A1 in zebrafish: Cloning, regulation and potential involvement in hyperactivitiy disorders. Toxicol. Appl. Pharmacol. 296, 73–84 (2016).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  39. 39.

    Takaku, Y. et al. Innexin gap junctions in nerve cells coordinate spontaneous contractile behavior in hydra polyps. Sci. Rep. 4, 3573. https://doi.org/10.1038/srep03573 (2014).

    ADS  Article  PubMed  PubMed Central  Google Scholar 

  40. 40.

    Elphick, M. R., Mirabeau, O. & Larhammar, D. Evolution of neuropeptide signaling systems. J. Exp. Biol. 221, 151092. https://doi.org/10.1242/jeb.151092 (2018).

    Article  Google Scholar 

  41. 41.

    Kusserow, A. et al. Unexpected complexity of the Wnt gene family in a sea anemone. Nature 433, 156–160 (2005).

    ADS  CAS  PubMed  Article  PubMed Central  Google Scholar 

  42. 42.

    Lengfeld, T. et al. Multiple Wnts are involved in Hydra organizer formation and regeneration. Dev. Biol. 330, 186–199 (2009).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  43. 43.

    Magie, C. R., Pang, K. & Martindale, M. Q. Genomic inventory and expression of SOX and FOX genes in the cnidarian Nematostella vectensis. Dev Genes Evol. 215, 618–630 (2005).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  44. 44.

    Steele, R. E., David, C. N. & Techanu, U. A genomic view of 500 million years of cnidarian evolution. Trends Genet. 27, 7–13 (2011).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  45. 45.

    Tarrant, A. M., Reitzel, A. M., Kwok, C. K. & Jenny, M. J. Activation of the cnidarian oxidative stress response by ultraviolet radiation, polycyclic aromatic hydrocarbons and crude oil. J. Exp. Biol. 217, 1444–1453 (2014).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  46. 46.

    Tarrant, A. M., Payton, S. L., Reitzel, A. M., Porter, D. R. & Jenny, M. J. Ultraviolet radiation significantly enhances the molecular response to dispersant and sweet crude oil exposure in Nematostella vectensis. Mar. Environ. Res. 134, 96–108 (2018).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  47. 47.

    Petrunak, E. M., DeVore, N. M., Porubsky, P. R. & Scott, E. E. Structures of human steroidogenic cytochrome P450 17A1 with substrates. J. Biol. Chem. 289, 32952–32964 (2014).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  48. 48.

    Pallan, P. S. et al. Human cytochrome P450 21A2, the major steroid 21-hydroxylase: Structure of the enzyme·progesterone substrate complex and rate-limiting C-H bond cleavage. J. Biol. Chem. 290, 13128–13143 (2015).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  49. 49.

    Nerbert, D. W., Wikvall, K. & Miller, W. L. Human cytochromes P450 in health and disease. Philos. Trans. R. Soc. Lond. B Biol. Sci. 368, 20120431. https://doi.org/10.1098/rstb.2012.0431 (2013).

    CAS  Article  Google Scholar 

  50. 50.

    Guo, H. et al. Identification of cytochrome P450 (CYP) genes in Zhikong scallop (Chlamys farreri). J. Ocean Univ. China 12, 97–102 (2013).

    ADS  CAS  Article  Google Scholar 

  51. 51.

    Han, J., Park, J. C., Hagiwara, A., Park, H. G. & Lee, J. S. Identification of the full 26 cytochrome P450 (CYP) genes and analysis of their expression in response to benzo[a]pyrene in the marine rotifer Brachionus rotundiformis. Comp. Biochem. Physiol. D 29, 185–192 (2019).

    CAS  Google Scholar 

  52. 52.

    Marlow, H. Q., Srivastava, M., Matus, D. Q., Rokhsar, D. & Martindale, M. Q. Anatomy and development of the nervous system of Nematostella vectensis, an anthozoan cnidarian. Dev. Neurobiol. 69, 235–254 (2009).

    CAS  PubMed  Article  Google Scholar 

  53. 53.

    Twan, W. H., Hwang, J. S. & Chang, C. F. Sex steroids in scleractinian coral, Euphyllia ancora: Implication in mass spawning. Biol. Reprod. 68, 2255–2260 (2003).

    CAS  PubMed  Article  Google Scholar 

  54. 54.

    Tarrant, A. M., Atkinson, M. J. & Atkinson, S. Estrone and estradiol-17 beta concentration in tissue of the scleractinian coral, Montipora verrucosa. Comp. Biochem. Physiol. A Mol. Integr. Physiol. 122, 85–92 (1999).

    CAS  PubMed  Article  Google Scholar 

  55. 55.

    Goldstone, J. V. et al. Genetic and structural analyses of cytochrome P450 hydroxylases in sex hormone biosynthesis: Sequential origin and subsequent coevolution. Mol. Phylogenet. Evol. 94(Pt B), 676–687 (2016).

    CAS  PubMed  Article  Google Scholar 

  56. 56.

    Lamb, D. C., Kelly, D. E. & Kelly, S. L. Molecular diversity of sterol 14α-demethylase substrates in plants, fungi and humans. FEBS Lett. 425, 263–265 (1998).

    CAS  PubMed  Article  Google Scholar 

  57. 57.

    Morrison, A. M. S. et al. Identification, modeling and ligand affinity of early deuterostome CYP51s and functional characterization of recombinant zebrafish sterol 14α-demethylase. Biochem. Biophys. Acta 1840, 1825–1836 (2014).

    CAS  PubMed  Article  Google Scholar 

  58. 58.

    Zhang, T. et al. Evolution of the cholesterol biosynthesis pathway in animals. Mol. Biol. Evol. 36, 2548–2556 (2019).

    CAS  Article  Google Scholar 

  59. 59.

    Nelson, M. M., Phleger, C. F., Mooney, B. D. & Nichols, P. D. Lipids of gelatinous Antarctic zooplankton: Cnidaria and ctenophora. Lipids 35, 551–559 (2000).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  60. 60.

    Kanazawa, A., Teshima, S. & Tomita, S. Sterol biosynthesis in some coelenterates and echinoderms. Bull. Jpn. Soc. Sci. Fish 40, 1257–1260 (1974).

    CAS  Article  Google Scholar 

  61. 61.

    Dermauw, W., Van Leeuwen, T. & Feyererisen, R. Diversity and evolution of the P450 family in arthropods. Insect Biochem. Mol. Biol. 127, 103490 (2020).

    CAS  PubMed  Article  Google Scholar 

  62. 62.

    Technau, U. & Schwaiger, M. Recent advances in genomics and transcriptomics of cnidarians. Mar. Genomics 24, 131–138 (2015).

    PubMed  Article  Google Scholar 

  63. 63.

    Hasemann, C. A., Kurumbail, R. G., Boddupalli, S. S., Peterson, J. A. & Deisenhofer, J. Structure and function of cytochromes P450: A comparative analysis of three crystal structures. Structure 3(1), 41–62 (1995).

    CAS  PubMed  Article  Google Scholar 

  64. 64.

    Werck-Reichhart, D. & Feyereisen, R. Cytochromes P450: A success story. Genome Biol. 1, 3003.1-3003.9. https://doi.org/10.1186/gb-2000-1-6-reviews3003 (2000).

    Article  Google Scholar 

  65. 65.

    Werck-Reichhart, D., Bak, S., & Paquette, S. Cytochrome P450. in The Arabidopsis Book e0028 (2002).

  66. 66.

    Baker, M. E., Nelson, D. R. & Studer, R. Origin of the response to adrenal and sex steroids: Roles of promiscuity and co-evolution of enzymes and steroid receptors. J. Steroid Biochem. Mol. Biol. 151, 12–24 (2014).

    PubMed  Article  CAS  Google Scholar 

  67. 67.

    Markov, G. V. et al. Independent elaboration of steroid hormone signaling pathways in metazoans. Proc. Natl. Acad. Sci. USA 106, 11913–11918 (2009).

    ADS  CAS  PubMed  Article  Google Scholar 

  68. 68.

    Altschul, S. F., Gish, W., Miller, W., Myers, E. W. & Lipman, D. J. Basic local alignment search tool. J. Mol. Biol. 215, 403–410 (1990).

    CAS  Article  Google Scholar 

  69. 69.

    Skinner, M. E., Uzilov, A. V., Stein, L. D., Mungall, C. J. & Holmes, I. H. JBrowse: A next generation genome browser. Genome Res. 19, 1630–1638 (2009).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  70. 70.

    Kent, W. J. BLAT – The BLAST-like alignment tool. Genome Res. 12, 656–664 (2002).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  71. 71.

    Finn, R. D. et al. The Pfam protein families database. Nucelic Acids Res. 38, D211–D222. https://doi.org/10.1093/nar/gkp985 (2010).

    CAS  Article  Google Scholar 

  72. 72.

    Sigrist, C. J. A., Cerutti, L. & de Castro, E. PROSITE, a protein domain database for functional characterization and annotation. Nucleic Acids Res. 38, D161–D166. https://doi.org/10.1093/nar/gkp885 (2010).

    CAS  Article  PubMed  Google Scholar 

  73. 73.

    Sievers, F. et al. Fast, scalable generation of high-quality protein multiple sequence alignments using Clustal Omega. Mol. Syst. Biol. 7, 539. https://doi.org/10.1038/msb.2011.75 (2011).

    Article  PubMed  PubMed Central  Google Scholar 

  74. 74.

    74Maddison, W. P., & Maddison, D. R. Mesquite: A Modular System for Evolutionary Analysis. Version 3.10 http://mesquiteproject.org (2016)

  75. 75.

    Stamatakis, A. RAxML version 8: A tool for phylogenetic analysis and post-analysis of large phylogenies. Bioinformatics 30, 1312–1313 (2014).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  76. 76.

    Rambaut, A. FigTree v1.4.3. http://tree.bio.ed.ac.uk/software/figtree/ (2016)

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Acknowledgements

This study was supported by grants from the Natural Science Engineering Research Council of Canada in the form of a Discovery Grant (RGPIN-328204-2011 and RGPIN-05767-2016) to J.Y.W. A.G.M. held a Cisco Research Chair in Bioinformatics, supported by Cisco Systems Canada, Inc. K.V.P. was supported by a Natural Sciences and Engineering Research Council of Canada (NSERC) Undergraduate Student Research Award (USRA). Computer resources were supplied by the McMaster Service Lab and Repository computing cluster, funded in part by grants to A.G.M. from the Canadian Foundation for Innovation (34531 to A.G.M.). The authors would like to thank Amos Raphenya and Brian Alcock (McMaster University) for assistance with computational tasks.

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Genome annotation of CYPs in Hydra, Acropora, and Aurelia genomes was completed by K.V.P.; J.V.G. completed the genome annotations in Nematostella. D.A.G. shared the Aurelia genome data for this study. Gene alignments, motif searching, phylogenetic analyses were completed by K.V.P. A.G.M. and J.Y.W. were co-supervisors of K.V.P. and contributed with K.V.P. to draft manuscript writing and editing; A.G.M. provided bioinformatics supports in terms of cluster access. D.R.N. provided the nomenclature assignment of all the genes based on sequence and phylogenies provided by K.V.P. and J.Y.W. Gene nomenclature was verified by J.V.G. and J.Y.W. The project idea and major funding was from J.Y.W. All co-authors contributed to writing and editing the manuscript.

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Correspondence to Joanna Y. Wilson.

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Pankov, K.V., McArthur, A.G., Gold, D.A. et al. The cytochrome P450 (CYP) superfamily in cnidarians. Sci Rep 11, 9834 (2021). https://doi.org/10.1038/s41598-021-88700-y

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