Cytosine methylation is a conserved epigenetic feature found throughout the phylum Platyhelminthes
- Kathrin K Geyer†1,
- Iain W Chalmers†1,
- Neil MacKintosh1,
- Julie E Hirst1,
- Rory Geoghegan1,
- Mathieu Badets2,
- Peter M Brophy1,
- Klaus Brehm3 and
- Karl F Hoffmann1Email author
© Geyer et al.; licensee BioMed Central Ltd. 2013
Received: 14 December 2012
Accepted: 3 July 2013
Published: 9 July 2013
The phylum Platyhelminthes (flatworms) contains an important group of bilaterian organisms responsible for many debilitating and chronic infectious diseases of human and animal populations inhabiting the planet today. In addition to their biomedical and veterinary relevance, some platyhelminths are also frequently used models for understanding tissue regeneration and stem cell biology. Therefore, the molecular (genetic and epigenetic) characteristics that underlie trophic specialism, pathogenicity or developmental maturation are likely to be pivotal in our continued studies of this important metazoan group. Indeed, in contrast to earlier studies that failed to detect evidence of cytosine or adenine methylation in parasitic flatworm taxa, our laboratory has recently defined a critical role for cytosine methylation in Schistosoma mansoni oviposition, egg maturation and ovarian development. Thus, in order to identify whether this epigenetic modification features in other platyhelminth species or is a novelty of S. mansoni, we conducted a study simultaneously surveying for DNA methylation machinery components and DNA methylation marks throughout the phylum using both parasitic and non-parasitic representatives.
Firstly, using both S. mansoni DNA methyltransferase 2 (SmDNMT2) and methyl-CpG binding domain protein (SmMBD) as query sequences, we illustrate that essential DNA methylation machinery components are well conserved throughout the phylum. Secondly, using both molecular (methylation specific amplification polymorphism, MSAP) and immunological (enzyme-linked immunoabsorbent assay, ELISA) methodologies, we demonstrate that representative species (Echinococcus multilocularis, Protopolystoma xenopodis, Schistosoma haematobium, Schistosoma japonicum, Fasciola hepatica and Polycelis nigra) within all four platyhelminth classes (Cestoda, Monogenea, Trematoda and ‘Turbellaria’) contain methylated cytosines within their genome compartments.
Collectively, these findings provide the first direct evidence for a functionally conserved and enzymatically active DNA methylation system throughout the Platyhelminthes. Defining how this epigenetic feature shapes phenotypic diversity and development within the phylum represents an exciting new area of metazoan biology.
The Platyhelminthes (flatworms) contain a diverse group of acoelomate, triploblastic organisms. While debate continues as to the evolutionary relationship of the 100,000 or so extant species within this phylum , the general consensus remains that these metazoans consist of four major clades: the monophyletic classes Cestoda (endoparasitic tapeworms), Monogenea (mostly ectoparasitic forms) and Trematoda (endoparasitic flukes) as well as the paraphyletic ‘Turbellaria’ (mostly free-living species). As tractable examples of development and self-regeneration (e.g. turbellarians and cestodes) or as causative agents of aquaculture, veterinary and biomedically-relevant parasitic diseases (e.g. monogeneans, trematodes and cestodes), the platyhelminths are an intensively studied invertebrate group. These research projects have fuelled numerous ‘omics’ investigations, which in turn, have yielded genetic information pertinent to our current understanding of platyhelminth development, parasite biology, metazoan evolution and adaptation. However, the likely considerable role of ‘epigenetics’-based mechanisms in the regulation of these diverse biological processes has yet to be fully investigated .
Epigenetics explains how heritable (and potentially reversible) changes in gene expression, caused by mechanisms that do not alter the underlying genetic code, contribute to phenotypic diversity within individuals of a population. Amongst the four major types of epigenetic processes (DNA methylation, histone modifications, miRNA mediated transcriptional regulation and nuclear gene repositioning) found within eukaryotes, DNA methylation is the most highly studied. DNA methylation affects phenotypic diversity by regulating allelic exclusion , gene expression , embryogenesis  and repetitive element silencing . Metazoan DNA methyltransferases (DNMT1, DNMT2, DNMT3a/3b ) catalyse this feature by transferring a methyl group (CH3) from S-adenosylmethionine (SAM) to the 5-carbon (C5) position of cytosine in gDNA. These ‘epigenetic marks’ are subsequently recognised by methyl-CpG binding domain proteins (MeCP2 and MBD1-4) and converted into signals necessary for generating phenotypic diversity . Together, DNMTs and MBDs (complexed with other proteins ) comprise the core metazoan DNA methylation system found in both vertebrate and invertebrate species.
Historically, DNA methylation was not thought to occur in the phylum Platyhelminthes. This belief was based on a small number of studies, which used rather imprecise methodologies or only sampled restricted developmental lifecycle stages or species [10–12]. However, by utilising a complementary suite of more sensitive technologies and surveying seven distinct lifecycle stages, Geyer et al. recently challenged this long-standing dogma in epigenetics and clearly demonstrated a functional role for DNA methylation in the developmental biology of S. mansoni. In this current investigation, we extend findings of S. mansoni DNA methylation to other representative platyhelminth species. We report, for the first time, that DNA methylation (on cytosine residues) and essential DNA methylation machinery components (DNMTs and MBDs) are indeed present in both parasitic and free-living flatworm species. The evolutionary conservation of this epigenetic mark in the developmental progression of monophyletic- (parasitic Cestoda, Monogenea and Trematoda) and paraphyletic – (free-living ‘Turbellaria’) platyhelminths [1, 14] that inhabit different ecological niches and employ diverse trophic strategies awaits further investigations.
The Platyhelminthes contain conserved DNMT2 DNA methyltransferases
As a phylum, the Platyhelminthes are predominantly studied due to their disease causing potential  and/or their suitability as models for investigating regenerative/stem-cell biology [16–18]. Recent genome sequencing- and functional genomics- efforts have led to rapid advances in our understanding of the molecular processes underpinning platyhelminth development, anthelmintic resistance, phenotypic plasticity and host interactions. However, the considerable role of epigenetic-based mechanisms contributing to these phenomena has yet to be fully investigated . Indeed, only recently has a function for cytosine methylation been demonstrated in the developmental biology of a platyhelminth species (S. mansoni; ). Here, a role in schistosome egg production was associated with the transcriptional co-regulation of key schistosome DNA methylation machinery components (SmDNMT2 and SmMBD) that mirrored the detection of genomic 5-methyl cytosine (5mC). Collectively, these data indicated that schistosomes encode a DNA methylation machinery responsible for epigenetic alterations to genome structure and that this process contains components functionally similar to those described in other eukaryotes . Therefore, to investigate whether DNA methylation is uniquely found within the Schistosoma or, rather, features as a conserved regulator driving genomic/phenotypic diversity within other parasitic or free-living platyhelminths, we conducted an investigation searching for essential epigenetic mediators (SmDNMT2/SmMBD homologs) and corresponding epigenetic marks (cytosine methylation) throughout the phylum.
Another invariant region found amongst the platyhelminth DNMT candidates is the glutamic acid/asparagine/valine tripeptide (E114/N115/V116 in SmDNMT2) of motif VI (Figure 1). Within this tripeptide, the glutamic acid residue utilises hydrogen bonding to interact with the target cytosine and is necessary for the stability of the enzyme/target complex . The motif VIII arginine (R157 in SmDNMT2) also facilitates hydrogen bonding to stabilise enzyme/cytosine complexes  and is, similar to SmDNMT2 E114, absolutely conserved across the representative platyhelminth DNMTs (Figure 1).
The presence of these six motifs (I, IV, VI, VIII, IX and X) within the C-terminal catalytic domain (PF00145) and the absence of DNMT1 and DNMT3 N-terminal regulatory domains strongly indicate that these new platyhelminth DNMTs are SmDNMT2 homologs. Additionally, conserved aspartic acid/isoleucine dipeptides (D254/I255 in SmDNMT2) and cysteine/phenylalanine/threonine tripeptides (C265/F266/T267 in SmDNMT2) within the TRD (between motifs VIII and IX) add further support to this assertion (Figure 1). These two polypeptide regions are specific to DNMT2 family members and are not found in DNMT1, DNMT3 or bacterial DNA methyltransferases. Importantly, the CFT tripeptide has been additionally proposed to help coordinate target recognition during enzyme interactions . Therefore, strong CFT conservation in all but one (S. mediterranea contains a T266 to I266 substitution in the CFT tripeptide) platyhelminth DNMT candidate further supports their inclusion as new DNMT2 family members. While vertebrate DNMT2 family members are now considered predominant tRNA methyltransferases , many invertebrate/single-cell eukaryote DNMT2s still retain strong DNA methyltransferase activity [31–34]. The enigmatic role and genomic targets of these new platyhelminth DNMT2s await enzymatic and functional characterisation.
The Platyhelminthes contain conserved MBD2/3 methyl-CpG binding proteins
Despite sharing greater than 70% amino acid identity, indicative of a gene duplication event , mammalian MBD2 is capable of binding methylated cytosine within gDNA whereas MBD3 is not . Therefore, identifying whether these new platyhelminth MBD2/3 proteins share greater sequence similarity to methyl-CpG binding MBD2 or non methyl-CpG binding MBD3 members was investigated. Specific attention was focused on amino acids known to be important for MBD function (i.e. binding to methyl-CpG) and included the following residues: arginine 58 (R58), lysine 66 (K66), tyrosine 79 (Y70) and arginine 80 (R80) (SmMBD2/3 numbering used unless otherwise stated; Figure 3, asterisks above PF01429 consensus sequence). Both K and Y residues are important for MBD function (e.g. Y residue coordinating H-bonding to 5mC ) as mammalian MBD3 contains K30 to H30 and Y34 to F34 substitutions (Figure 3) and is unable to bind methylated cytosine . In addition, both R residues also are critical in MBD/target (5mC) interactions as demonstrated by recent X-ray crystallography studies [42, 43]. Whereas all platyhelminth MBD2/3s contain conserved K66 and R80 residues, there is variability in the conservation of SmMBD2/3 Y70 and R58 residues. For example, the Y70 amino acid position is maintained in SmMBD2/3, SjMBD2/3, CsMBD2/3 and OvMBD2/3, but is substituted for an F in P. westermani MBD2/3 and all of the cestode sequences (E. multilocularis, T. solium, H. microstoma and E. granulosus). Furthermore, in S. mediterranea SmdMBD2/3, M. lignano MlMBD2/3 and H. microstoma HmMBD2/3 sequences, a R to K substitution at position 58 is also observed (Figure 3). Based on structural and comparative studies, both of these substitutions likely affect the methyl-CpG binding ability of P. westermani, S. mediterranea M. lignano and cestode MBD2/3 proteins  and may indicate additional/altered functions of these platyhelminth members (perhaps similar to MBD3L1/MBD3L2 , MBD3  or other MBD2/3 [46, 47] homologs). For SmMBD2/3, SjMBD2/3, CsMBD2/3 and OvMBD2/3 members, containing the full repertoire of functionally-conserved amino acid residues in their methyl-CpG binding domains, it is likely that these proteins bind 5mC. However, as shown for Drosophila melanogaster MBD2/3 , 5mC recognition of these platyhelminth members may be predominantly in the CpT/CpA context. Evidence to support this contention was recently provided in S. mansoni, where cytosine methylation was predominantly found in the CpA context [12, 13]. Clearly, further investigations are necessary to extend this locus-specific observation and identify the repertoire of activities mediated by platyhelminth MBD2/3 proteins.
DNA methylation is found in all four platyhelminth classes
We next used MSAP to identify cytosine methylation in E. multilocularis (containing EmDNMT2, Figures 1 and 2) protoscoleces and P. xenopodis (monogenean parasite related to NmDNMT2-containing N. mellini, Figures 1 and 2) adults obtained from the urinary bladder of infected X. laevis (Figure 5A). Discrete segregation (between MspI and HpaII digested populations) along the first principal coordinate indicated clusters of genomic loci containing this epigenetic modification in both parasitic platyhelminths. Importantly, this is the first molecular evidence for global cytosine methylation in the genomes of both Cestoda and Monogenea species. In contrast to E. multilocularis and P. xenopodis genomes, we were unable to confidently extend MSAP to detect cytosine methylation in F. hepatica (hermaphroditic trematode related to dioecious schistosomes) and P. nigra (turbellarian related to SmdDNMT2-containing S. mediterranea or MlDNMT2-containing M. lignano, Figures 1 and 2) genomes (collected from individual worms). Despite the suggestion of MSAP-detectable DNA methylation in these two species (HpaII and MspI populations are generally separated, Additional file 1), the presence of genetic diversity amongst sampled replicates averts the inference of epigenetic distance. The genetic diversity manifested itself in parasite MspI (methylation insensitive enzyme; indicative of genomic homozygosity/heterozygosity) populations contributing to more variability than parasite HpaII (methylation sensitive enzyme; indicative of methylated genomic loci) populations during multivariate analysis (Additional file 1). The environmental sources of both F. hepatica (sheep from different provenances) and P. nigra (rocky shores of Llyn-yr-Oerfa) led to sampling of outbred individuals and likely accounted for this genetic diversity.
Therefore, to survey for 5mC in these particular platyhelminth species, an alternative method for detecting 5mC was employed (Figure 5B). This involved an ELISA-based approach, which also was used to successfully identify 5mC in S. mansoni and M. musculus. Using this methodology, 5mC was found in both E. multilocularis and P. xenopodis genomes (Figure 5B), confirming the MSAP results for these parasites (Figure 5A) and providing confidence that ELISA-based detection of this genome modification could be translated from Schistosoma to other platyhelminth genomes. When subsequently applied to P. nigra and F. hepatica genomes, clear evidence for 5mC was obtained (Figure 5B). While not exhaustive, this ELISA-based study suggested that digenean trematodes (F. hepatica) contain higher levels of 5mC when compared to representative cestode- (E. multilocularis), monogenean- (P. xenopodis) and turbellarian- (P. nigra) species. Quantitative detection of 5mC in additional platyhelminth species (across the four classes within the phylum) would help to clarify this observation.
The combined presence of conserved DNMT2 and MBD2/3 candidates, as well as cytosine methylation marks throughout the Platyhelminthes, suggests that epigenetic-mediated DNA methylation features in the complex biology of this important phylum. However, it remains to be determined if all species within this phylum have maintained this epigenetic trait or, similar to the Arthropoda [34, 50–54] and Nematoda , some platyhelminths (especially within the paraphyletic ‘Turbellaria’ ) have lost this inheritable mechanism for generating phenotypic diversity. Furthermore, identifying the full enzymatic and target specificities of platyhelminth DNMT2 homologs requires additional investigation. It is currently unknown whether platyhelminth DNMT2s, in addition to DNA, have an affinity for tRNA substrates . Also, the only study to investigate DNA methylation at single base pair resolution within the Platyhelminthes has produced ambiguous results likely due to sampling of S. mansoni adult male gDNA only . In previous studies this schistosome developmental form has been shown to contain the lowest level of cytosine methylation throughout the parasite’s lifecycle . Future work will help characterise additional roles of platyhelminth DNMT2s and lead to the identification of genomic positions (e.g. repetitive elements, coding/non-coding genomic loci) targeted by this core DNA methylation machinery component. By doing so in a comprehensive manner (elucidation of DNA methylomes from various lifecycle stages and different platyhelminth species), insights into regenerative-, stem cell- and developmental-biology will be obtained leading to both a greater understanding of the complex life histories within the Platyhelminthes and novel opportunities for control.
Animal handling, care and subsequent experimentation were performed in compliance with German (Deutsches Tierschutzgesetz,TierSchG, version from Dec-9-2010) and European (European directive 2010/63/EU) regulations on the protection of animals. Ethical approval of the study was obtained from the local ethics committee of the government of Lower Franconia (Regierung von Unterfranken 55.2-2531.01-31/10).
Platyhelminth material and gDNA isolation
Mixed sex, adult S. japonicum and S. haematobium worms (blood flukes, class Trematoda) were obtained from perfusion of infected mice and hamsters, respectively . Adult F. hepatica worms (liver flukes, class Trematoda) were carefully removed from livers and bile ducts of naturally infected sheep (collected from Randell Parker Foods, Llanidloes, Wales). These parasites were washed six times in pre-warmed (37°C) phosphate buffered saline (PBS, pH 7.3) and cultured (one adult/well in a six well tissue culture plate) in DMEM (Sigma-Aldrich, UK) supplemented with 10% foetal calf serum, 2 mM L-glutamine, 100 U/ml penicillin and 100μg/ml streptomycin in an atmosphere of 5% CO2 for 48 hr with a 70% media exchange performed after 24 hr. P. xenopodis (class Monogenea) adult worms were collected from urinary bladders of infected X. laevis originating in Potchefstroom, South Africa. P. nigra (class Turbellaria) were collected from stones at the edges of Llyn-yr-Oerfa (Mid Wales) and maintained in a cold-water aquarium for 6 days without food. JAVA, a natural E. multilocularis isolate from the liver of an infected cynomolgus monkey (Macaca fascicularis; ) was passaged intraperitoneally through laboratory jirds (Meriones unguiculatus; ). E. multilocularis genomic DNA (gDNA) was isolated from a pure protoscolex preparation  after treatment with pepsin at pH 2  according to a previously established protocol . The remaining platyhelminth gDNA samples were extracted using the Qiagen DNeasy Kit. All gDNA samples were subsequently quantified by a Nanodrop-1000 spectrophotometer. Where possible (S. japonicum, F. hepatica, P. xenopodis and E. multilocularis), gDNA was subjected to host-contamination checks by PCR as previously described [13, 62] (Additional file 2).
Platyhelminth DNMT2 and MBD sequence identification
DNMT2 and MBD members from platyhelminth species were identified by tBLASTn searches of transcripts, predicted genes and genome assemblies of NCBI , Welcome Trust Sanger Institute  and Gasser Laboratory  EST databases as well as T. solium, S. mediterranea (SmedGD v1.3.14; ), M. lignano and F. hepatica gene models/genomic databases using SmDnmt2 IsoformI (NCBI accession no. HM991456) and SmMBD (NCBI accession no. HM991455) as query sequences. A Pfam domain search on SchistoDB v3.0 (beta version; ) was performed to identify a DNMT homolog within the genome of S. haematobium. Searches were performed on 25-01-12 for S. japonicum, S. haematobium, P. westermani, C. sinensis, O. viverrini, N. melleni and S. mediterranea, 14-11-12 for F. hepatica and M. lignano and 01-05-13 for E. granulosus, E. multilocularis, T. solium and H. microstoma. Where multiple ESTs (or ESTs and gene predictions) existed of the same homolog, a consensus sequence was formed. In the cases of S. haematobium, M. lignano, F. hepatica, E. multilocularis, E. granulosus, H. microstoma and T. solium DNMT homologs, the exon-intron structure of SmDNMT2 IsoformI was used as a reference to identify/correct the platyhelminth DNMT prediction. All exon/intron junctions in these altered gene predictions conformed to the consensus (GT/AG) splice donor/acceptor sequences for eukaryotes. Final amino acid sequences used in the study are listed in Additional file 3.
Sequence alignments and phylogenetic trees
Multiple sequence alignments of platyhelminth DNMT and MBD candidates were generated using MUSCLE v3.8 . Domain predictions were performed using the Pfam web server  to define the limits of the C-5 cytosine-specific DNA methylase domain (DNMT; PF00145), Methyl-CpG binding domain (MBD; PF01429) and C-terminal domain of methyl-CpG binding protein 2 and 3 (MBD_C; PF14048) regions for each sequence. Motif positions represented in the DNMT multiple sequence alignment were derived from a previous report . In addition to the identified platyhelminth candidates, the following sequences were included in the multiple sequence alignments as representative DNMT and MBD members: M. musculus MBD2 (NM_010773), M. musculus MBD3 (NM_013595), Pristionchus pacificus MBD2/3 (AAV85979.1), M. musculus DNMT2 (AAC53529.1) and S. pombe DNMT2 (CAA57824.1).
For phylogenetic analysis (using Maximum Likelihood and Bayesian approaches) of platyhelminth and non-platyhelminth DNMT members, amino acid sequences were aligned using MUSCLE software with minor improvements in the alignment performed following visual inspection. Non-conserved regions were then removed from the alignment to allow for phylogenetic comparison (during this step the target recognition domain (TRD) and variable regions were removed). In total, 230 amino acid positions were used in the analyses. The non-platyhelminth sequences (and their NCBI accession numbers) included in the DNMT phylogenetic analyses were as follows: M. musculus DNMT1 (P13864.5), M. musculus DNMT2 (AAC53529.1), M. musculus DNMT3a (O88508.2), M. musculus DNMT3b (O88509.2), A. mellifera DNMT1 (NP_001164522.1), A. mellifera DNMT2 (XP_393991.3), A. mellifera DNMT3 (NP_001177350.1), C. intestinalis DNMT2 (XP_002128135.1), C. intestinalis DNMT1 (XP_002122948.1), C. intestinalis DNMT3a (XP_002123461.1), Culex quinquefasciatus DNMT2 (XP_001867327.1), B. mori DNMT1 (NP_001036980.1), C. teleta Dnmt1a (ELT93682.1), C. teleta Dnmt1b (ELU12454.1), C. teleta Dnmt2 (ELU13416.1), C. gigas Dnmt2 (EKC25033.1), L. gigantea Dnmt1 (transcript name: 114987 ) L. gigantea Dnmt2 (transcript name: 119453 ), L. gigantea Dnmt3 (transcript name: 171288 ), H. robusta (transcript name: 116156 ), H. robusta Dnmt2 (transcript name: 89038 ) and H. robusta Dnmt3 (transcript name: 162653 ). The Bayesian phylogenetic analyses were performed as described previously  using MrBayes v3.1.2 , the WAG substitution model  and a minimum of 1 million generations. The log-likelihood score of each saved tree was plotted against the number of generations to determine the point at which the log-likelihood scores of the analyses stabilised. Maximum Likelihood analysis was conducted using MEGA 5.0  with the WAG substitution model and 1000 bootstrap replicates. The graphical output of the final Bayesian consensus phylogram was obtained using Figtree v1.3.1 . This tree was then exported into Adobe Illustrator where Maximum Likelihood bootstrap support values for each node were superimposed.
Phylogenetic analyses of the MBD proteins were performed using a MUSCLE alignment restricted to the MBD domain regions of the sequences (as defined by Pfam; PF01429). The non-platyhelminth sequences (and their NCBI accession numbers) included in the MBD phylogenetic analyses were as follows: M. musculus MBD1 (NM_013594), M. musculus MBD2 (NM_010773), M. musculus MBD3 (NM_013595), M. musculus MBD4 (NM_010774), M. musculus MeCP2 (NM_010788), X. laevis MBD1 (NP_001104183.1), X. laevis MBD2 (NP_001083787.1), X. laevis MBD3 (BAC22082.1), X. tropicalis MBD4 (NP_001037916.1), X. laevis MeCP2 (AAD03736.1), H. pulcherrimus MBD2/3 (EU590662), B. mori MBD2/3 (BGIBMGA001425-PA; SilkDB ), C. teleta MBD2/3 (ELT95247.1), C. gigas MBD2/3 (EKC32831.1), L. gigantea MBD2/3 (transcript name: 112523 ) and H. robusta MBD2/3 (transcript name: 185546 ). Phylogenetic relationships between the 20 members were then inferred in the same way as for the DNMT homologs, using Maximum Likelihood and Bayesian approaches. Maximum Likelihood bootstrap support values for each node (in parentheses) were superimposed onto the Bayesian consensus phylogram using Adobe Illustrator.
Methylation specific amplification polymorphism (MSAP) analysis of platyhelminth CpG methylation
The MSAP method , modified for the detection of CpG methylation in S. mansoni, was applied to platyhelminth gDNA samples free from host contamination (Additional file 2). Five biological replicates were analysed for P. xenopodis (single adults), F. hepatica (single adults), P. nigra (single adults), S. haematobium (mixed-sex adults) and S. japonicum (mixed-sex adults) samples. Five technical replicates were examined for E. multilocularis protoscolex samples. Following amplicon size determination on an ABI 3100 DNA capillary sequencer (IBERS, Aberystwyth), the raw data was viewed and analysed in GeneMapper® v4.0. GenAlex v6.4 was subsequently employed for multivariate Principal Coordinate Analysis (PcoA).
ELISA detection of 5mC
The amount of 5mC in 100 ng of selected platyhelminth gDNA samples was analysed using the SuperSense Methylated DNA Quantification Kit (Epigentek) as previously described . Reactions were carried out in triplicates for each platyhelminth sample (P. nigra, F. hepatica, P. xenopodis and E. multilocularis) and in duplicates for the negative and positive control (both supplied with the kit). Fluorescent readings (530ex/590emnm) were obtained using a POLARstar Omega (BMG Labtech, UK) microtiter plate reader and samples were subsequently normalised to controls. The mean of the fluorescent readings obtained from the negative control sample was subtracted from the platyhelminth and positive control values. Subsequently, the fluorescent mean of the positive control values was set at 100% (5mC=100%), and the 5mC abundance in each platyhelminth sample was normalised to this value.
This work was supported by an IBERS PhD studentship awarded to KKG and a BBSRC grant (BB/K005448/1) awarded to KFH. We thank Dr. Fred Lewis at the Biomedical Research Laboratory for provision of S. japonicum and S. haematobium parasites (NIH-NIAID schistosome supply contract HHSN272201000005I) and Dr Joseph Jackson (IBERS, Aberystwyth University) for supply of X. laevis gDNA. We also thank members of the Hoffmann laboratory (Dr. Emily Peak, Dr. Martha Truscott and Ms Sabrina Munshi), Professor Mike Wilkinson (University of Adelaide), Dr. Carlos M. Rodríguez López (University of Adelaide) and Dr Russell Morphew (IBERS, Aberystwyth University) for many helpful discussions throughout this project. We additionally thank the Parasite Genomics group at the Wellcome Trust Sanger Institute for assistance with gene prediction searches of the E. multilocularis, E. granulosus and H. microstomum genomes. Finally, we thank the Developmental Biology and Stem Cell Research group at the Hubrecht Institute and the Helminth Genomics group at Liverpool University for the unpublished Macrostomum lignano and Fasciola hepatica genome sequences used in this study [64, 65].
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