Large genome size, including immense repetitive and non-coding fractions, still present challenges for capacity, bioinformatics and thus affordability of whole genome sequencing in most amphibians. Here, we test the performance of a single transcriptome to understand whether it can provide a cost-efficient resource for species with large unknown genomes. Using RNA from six different tissues from a single Palearctic green toad (Bufo viridis) specimen and Hiseq2000, we obtained 22,5 Mio reads and publish >100,000 unigene sequences. To evaluate efficacy and quality, we first use this data to identify green toad specific candidate genes, known from other vertebrates for their role in sex determination and differentiation. Of a list of 37 genes, the transcriptome yielded 32 (87%), many of which providing the first such data for this non-model anuran species. However, for many of these genes, only fragments could be retrieved. In order to allow also applications to population genetics, we further used the transcriptome for the targeted development of 21 non-anonymous microsatellites and tested them in genetic families and backcrosses. Eleven markers were specifically developed to be located on the B. viridis sex chromosomes; for eight markers we can indeed demonstrate sex-specific transmission in genetic families. Depending on phylogenetic distance, several markers, which are sex-linked in green toads, show high cross-amplification success across the anuran phylogeny, involving nine systematic anuran families. Our data support the view that single transcriptome sequencing (based on multiple tissues) provides a reliable genomic resource and cost-efficient method for non-model amphibian species with large genome size and, despite limitations, should be considered as long as genome sequencing remains unaffordable for most species.
Citation: Gerchen JF, Reichert SJ, Röhr JT, Dieterich C, Kloas W, Stöck M (2016) A Single Transcriptome of a Green Toad (Bufo viridis) Yields Candidate Genes for Sex Determination and -Differentiation and Non-Anonymous Population Genetic Markers. PLoS ONE 11(5): e0156419. https://doi.org/10.1371/journal.pone.0156419
Editor: Ulrich Joger, State Natural History Museum, GERMANY
Received: March 10, 2016; Accepted: May 15, 2016; Published: May 27, 2016
Copyright: © 2016 Gerchen et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: Data are available on GenBank (Biosample SAMN03993917) and in the Supporting Information of this paper.
Funding: This work was funded by DFG, STO493/2-2, STO493/3-1, Open Access Fund of the Leibniz Association.
Competing interests: The authors have declared that no competing interests exist.
Rare availability of amphibian genomes
The availability of whole genome sequencing has greatly facilitated evolutionary studies in non-model organisms . Besides comparative research involving entire genomes (e.g. ), applications include candidate gene approaches and the development of specific marker sets for population genetics and speciation research. However, for some groups of non-model organisms, like most amphibians with very high DNA content , whole genome sequencing still is bioinformatically challenging and costly, and very few complete genomes are available. Due to their large proportion of repetitive sequences, assembly and proper annotation of such genomes remain difficult. Currently only two assembled and annotated amphibian genomes have become available: that of the model anuran, the tropical clawed frog, Xenopus tropicalis (Pipidae) , and recently that of the Tibetan frog, Nanorana parkeri (Dicroglossidae) .
Transcriptome sequencing as genomic resource for large-genome non-model species
Genetic and genomic applications often involve candidate gene approaches, in which the role of genes, known from related or model species, is examined in association studies for non-model species. In taxa with huge, unknown genomes, where whole genome sequencing still remains unaffordable, a useful resource may be transcriptomics (e.g. ). As transcriptomes only include exons and UTRs, sequencing efforts can be restricted to a small portion of the genome, and thus to the exclusion of hard-to-assemble non-coding intronic and intergenic repetitive regions. Amphibian transcriptomic information is expected to be well-annotatable. Given that many restrictions for whole genome approaches include most amphibians, in the present paper, we aimed at testing the usefulness of a single anuran transcriptome for obtaining a list of candidate genes on sexual development and sex determination.
As another application, we aimed at the targeted development of non-anonymous transcriptomic microsatellites [7, 8], namely sex-specific and sex-linked markers. They appear less susceptible to phylogenetic noise than SNPs  and are applicable to population genetics and to study inheritance patterns [10, 11].
As our target species, we have chosen a diploid bufonid toad, the European green toad Bufo viridis. Importantly, no genome or transcriptome of the species or of related taxa from this systematic anuran family have so far been characterized. Palearctic green toads (B. viridis subgroup) form a complex of at least 12 mitochondrial lineages that inhabit large parts of Europe, North Africa and Asia with several diploid clades as well as tri- and tetraploid lineages . Multiple natural hybrid zones of lineages with different divergence time can be found in this group [13, 14], making it a highly attractive amphibian radiation to study speciation and sex chromosome evolution under diploid  and polyploid hybridization . In this paper, we present 11 markers located on the sex chromosome (with sex-linkage proven for 8 markers) and 10 autosomal markers for the B. viridis subgroup, most of which are transcriptome based and polymorphic.
Material and Methods
Animal sampling / ethics statement
Our study was approved by the relevant Institutional Animal Care and Use Committee (IACUC), namely the Service de la Consommation et des Affaires Vétérinaires du Canton de Vaud (Epalinges, Switzerland); toads and/or clutches were sampled according to permit 115790/229 in accordance with the Swiss import permit of the Bundesamt für Veterinärwesen, BVET Nr. 812/11, Bern, Switzerland, and authorization No. 1798, Service de la consommation et des affaires vétérinaires, Canton de Vaud, Epalinges, Switzerland.
Sequencing of a single transcriptome
RNA was extracted from six different tissues (liver, eye, brain, testes, heart, muscle) of a single male Bufo viridis, caught south of Astros, Greece (37.38299 N, 22.7455 E) in March 2011. RNA was pooled and adjusted to equal concentrations. Complementary DNA (cDNA) was synthesized and sequenced by BGI (BGI-Hongkong Co., Ltd.), using the Hiseq2000 sequencing system (Illumina, San Diego, USA). Reads were assembled using SOAPdenovo : contigs (longest assembled sequences without Ns) were linked into scaffolds by mapping reads back to contigs and combining paired-end information. Scaffold length was estimated according to the average segment length of each pair of reads, and unknown bases were filled with Ns. Gaps in scaffolds were filled using paired-end reads, resulting in so-called unigenes. Raw reads were transmitted to the NCBI Sequence Read Archive (SRA, http://www.ncbi.nlm.nih.gov/Traces/sra/) under the accession Number SRS1034407, assembled sequences were transmitted to NCBI Transcriptome Shotgun Assembly Sequence Database (TSA, http://www.ncbi.nlm.nih.gov/genbank/tsa), BioSample accession for the project is SAMN03993917.
Functional annotation and classification
To predict protein functional information from the annotation of blast hits, unigene sequences were searched against four protein databases (Nr, Swissprot, KEGG, COG) using Blastx  with an E-value threshold of E-05. Blast2GO  as applied for GO annotation on the basis of the results of the Nr annotation. GO functional classification of all unigenes was performed using WEGO .
Genes involved in sex determination or sex differentiation
To evaluate the usefulness of a single, though multiple tissue-based, amphibian transcriptome for candidate gene approaches, we aimed at retrieving genes involved in male or female sex determination and sexual differentiation (list from M. Schartl, pers. comm., modified for anurans). Template sequences from the anuran model species Xenopus tropicalis or X. laevis were retrieved from Xenbase . Sequences were blasted against a local database of all B. viridis unigenes using tblastn . Using NCBI blastn, homology of unigenes from the resulting blast hits was confirmed. Only best blast hits with an E-value lower than E-05 were considered homologous. Blast hits were not considered homologous when there were other blast hits for different genes with E-values less then 10000 times larger.
Development of transcriptome-based microsatellite markers
Despite 150 million years (My) of divergence between bufonid, hylid and ranid anurans, chromosome number and interphase banding patterns suggest a high degree of structural conservation of their genomes . Even after 200 My of separation, homology between large parts of X. tropicalis chromosome 1 (in which it is not the sex chromosome) and the sex chromosome of all examined diploid species of the B. viridis subgroup has been shown [15, 23]. Lacking more closely related relatives, the genome of X. tropicalis (and X. laevis) served as reference for B. viridis. Transcriptome data were first searched for microsatellite-like repetitive sequences (SSRs) using Misa (MIcroSAtellite identification tool, URL: http://pgrc.ipk-gatersleben.de/misa/). Repeats were filtered to exclude short repeats and duplicate entries. Sequences of repeat-containing unigenes were searched against the transcriptome of X. tropicalis  using the local alignment software Blast+ 2.2.25  with the options "–evalue = 0.01 and –task = blastn" to identify homologous transcripts in X. tropicalis. The resulting best blast hits (gene name abbreviations) were searched against a mapping file (a list of gene names, synonyms and abbreviations, X. tropicalis start and end position and length in bp) available from Xenbase , which allowed assignment to a specific gene and its genomic location in the X. tropicalis-genome. Different markers were then selected over the whole length of X. tropicalis linkage group 1. For comparative studies of sex chromosomes and autosomes, additional markers on several autosomal linkage groups were developed.
Because of the relatively low degree of polymorphisms in transcriptomic repeat sequences , different strategies were applied to increase the amount of polymorphic markers among candidates. Using Blast+  with the megablast algorithm, candidate unigene sequences were searched against a database of the raw B. viridis Illumina reads. The sequences of the resulting Blast hits were mapped onto the unigene sequence using Geneious 7.06 (Biomatters). Ambiguities represented by a ratio of about 50%: 50% of raw Illumina reads in the resulting alignment were interpreted as heterozygous alleles in the individual diploid genome, from which the transcriptome was generated. It was expected, that markers, which were polymorphic within the single individual were likely to differ also between lineages. Furthermore, Serv  was applied, an algorithm, which uses a nonlinear model to calculate a numeric VARscore from intrinsic sequence properties. The VARscore predicts repeat variability and sequences, which were not already polymorphic within the single transcriptome, were selected for a high VARscore. Intron-exon boundaries of the repeat-containing unigenes were determined using the X. tropicalis genome  for these candidate genes using the Ensembl genome browser . As amplification of genomic DNA markers fails if intron lengths and positions are not taken into account, X. tropicalis exons were aligned to the B. viridis unigene sequences using Geneious. PCR-primers for suitable marker candidates were then developed using Primer3 . Primers were tested in 10 μl gradient PCR-reactions containing 1 μl B. viridis (or other green toads’) DNA (10 ng/μl), 1 μl 10x TopTaq-PCR-Buffer (with 15 mM MgCl2; Qiagen), 1 μl dNTP-Mix (2.5 mM of each dNTP), 0.5 μl forward primer (10 pmol/μl), 0.5 μl reverse primer (10 pmol/μl), 0.05 μl TopTaq polymerase (Qiagen) and 5.95 μl RNAse free water. The PCR protocol reads: initial denaturation at 95°C for 3 min, 35 cycles (including denaturation at 94°C for 30 s, annealing at 48–68°C for 60 s and elongation at 72°C for 40 s), and final elongation at 72°C for 10 min. PCR-products were screened for optimal annealing temperatures using agarose (2%) gel electrophoresis. Markers were tested for polymorphisms by direct sequencing of PCR-products and at least five individuals of four green toad species (B. viridis, B. balearicus, B. siculus and B. variabilis) were genotyped. For sequencing reactions, 25 μl PCR reactions were conducted, containing 2.5 μl DNA (10 ng/μl), 2.5 μl 10x TopTaq-PCR-Buffer (with 15 mM MgCl2; Qiagen), 2.5 μl dNTP-Mix (2.5 mM of each dNTP), 1.25 μl forward primer (10 pmol/μl), 1.25 μl reverse primer (10 pmol/μl), 0.125 μl TopTaq polymerase (Qiagen) and 14.875 μl RNAse free water. The PCR-protocol comprised initial denaturation at 95°C for 3 min, 35 cycles (including denaturation at 94°C for 30 s, annealing at optimal annealing temperature for 60 s and elongation at 72°C for 40 s), and a final elongation at 72°C for 10 min.
PCR-products were purified and Sanger sequenced by Eurofins MWG (Ebersberg, Germany) using one or both of the original PCR primers for sequencing reactions. Sequences were aligned to the transcriptomic unigene sequences using Geneious and manually checked for indels, i.e. desired length polymorphisms.
Tests for sex linkage
To test whether markers located on X. tropicalis linkage group 1 are really located on the largely homologous B. viridis sex chromosome, sex-specific transmission was analyzed. In an XY-sex determination system, the father’s Y chromosome is always transmitted to male, while the X chromosome is always transmitted to female offspring. This was tested by genotyping previously generated genetic families with parents and offspring of known phenotypic sex [27, 28, 13]. Genotyping of all PCR-products was performed on an ABI 3500xL capillary sequencer (Applied Biosystems) with 0.5 μl diluted PCR-products in 9.25 μl Hi-Di formamide (Applied Biosystems) and 0.25 μl GeneScan 500 ROX size standard (Life Technologies). Genotypes were scored using Genemapper 4.1 (Applied Biosystems). Forward Primers of genotyping reactions were fluorescently labeled.
For markers BvCamk4 (ATTO-550 labeled), BvHNRNPD (FAM), BvCherp (ATTO-550), BvDMRT1 (HEX), BvVLDLR (HEX) and BvIno80b (HEX) genotypes of parents and offspring (28 females, 21 males) of B. balearicus x B. siculus-F1 Cr13 (father) and B. balearicus Si337 (mother) were genotyped. For markers BvEll2 (FAM) and BvGar1 (HEX) B. balearicus Si336 (father) and B. siculus Si335 (mother; ) and resulting offspring (n = 30) were genotyped. Because the phenotypic sex of this offspring was unknown, it was also genotyped with the classical microsatellite markers C223, known to be sex-linked in B. siculus and B. balearicus . C223 was amplified using 4 μl RNAse free water, 3 μl Multiplex PCR kit master mix (Qiagen), 0.5 μl C223 forward primer (10 pmol/μl, FAM-labeled), 0,5 μl C223 reverse primer (10 pmol/μl) and 2 μl DNA (10 ng/μl). The PCR-protocol comprised: Initial denaturation at 95°C for 15 min, 35 cycles (denaturation at 94°C for 30 s, annealing at 55°C for 90 s and elongation at 72°C for 60 s), and final elongation was at 60°C for 30 min. 0.5 μl of the C223 PCR-products were diluted in 22 μl RNAse free water and genotyped. Marker BvChd1 is nested in the same intron for, which sex linkage has been shown .
Cross-amplification was tested for 11 markers located on X. tropicalis linkage group 1 (S3 Table). PCRs were performed with single high-molecular DNA samples of verified quality and quantity from nine systematic anuran families, namely Allobates femoralis (Arombatidae), Bombina orientalis (Bombinatoridae), Bufo bufo, Rhinella marina (Bufonidae), Hyla arborea (Hylidae), Hyloxalus azureiventris (Dendrobatidae), Pelophylax esculentus, Rana temporaria (Ranidae), Pelobates fuscus (Pelobatidae) and Xenopus tropicalis (Pipidae). Gradient-PCRs ranging in annealing temperatures from 47.8°C to 68°C were performed to determine the optimum. In case of uncertainties about quality, quantity or specificity of products, PCRs were repeated using a narrower gradient around the assumed optimal target temperature.
Cross-amplification was tested in 10 μl gradient PCR-reactions containing 2 μl DNA (10 ng/μl), 1 μl 10x TopTaq-PCR-Buffer (with 15 mM MgCl2, Qiagen), 1 μl dNTP-Mix (2.5 mM of each dNTP), 1 μl of 10x CoralLoad Concentrate (Qiagen), 1 μl of 5x Q-Solution (Qiagen), 0.4 μl of MgCl2 (25mM, Qiagen), 0.5 μl of each primer (10 pmol/μl), and 0.05 μl TopTaq polymerase (Qiagen) and 2.55 μl RNAse free water. We considered markers to be specific when gel electrophoresis showed a clear band in proximity to the fragment size of B. viridis used as positive control on the same gel with 1 kb DNA HyperLadder (Bioline). Double or multiple bands and much larger or smaller bands suggested unspecific amplification. If a band in the right size could be determined among multiple bands the marker was declared as inoperable. To determine exact marker sequences in B. bufo, we used the conditions described above for green toad sequences. Sequences of the markers which could be successfully cross-amplified in B. bufo were aligned to the B. viridis unigene using sequences homologous to X. tropicalis-LG1-genes. Mapping of the sequences was done in Geneious 7.0.6.
Amplification success versus divergence time
To test inverse correlation of amplification success and evolutionary divergence, we took the divergence times of systematic anuran families from www.timetree.org. Amplification success is measured by the proportion of markers that amplified in each species to the total number of tested markers (S3 Table) developed for B. viridis. Maximum amplification success would be 10 out of 10 markers. Because of the proportional nature of the data, we calculated a generalized linear model (GLM) with binomial errors and a logit link (ANOVA, χ2). Statistical analysis was carried out in R version 3.1.0 .
The complete transcriptome data comprise 22,421,688 reads with a total length of 2,242,168,800 bp. The GC-content of the reads was 46.83%, 92.33% of all bases had a quality score of at least Q20. Assembly and scaffolding resulted in 110264 unigenes with a total length of 45,245,144 bp. Unigenes had an average length of 411 bp and a N50 of 504 bp. A total of 86707 unigenes ranged in length from 150 to 7508 bp (S1 Fig)
Sequence annotation revealed significant similarities to a large number of proteins from four protein databases (Table 1). Based on blast hits of the Nr database, 10541 unigenes (9.56%) were assigned to gene ontology terms.
Regarding the molecular function ontology, the most common classifications were cellular processes (8156), metabolic processes (6713) and biological regulation. The most common categories for the cellular component ontology were cellular (10437), cell compartments (9976) and organelles (6529). In terms of the molecular function, most common categories involved binding (7609), catalytic activity (4663) and molecular transducer activity (897) (S2 Fig).
Genes involved in sex determination or sex differentiation
Of a list 37 genes, ca. 87% (32) had significant blast hits in the B. viridis transcriptome, many of which providing the first sequence data for these genes in this non-model anuran species.
Compared to the length of Xenopus mRNAs used as BLAST templates, the majority of the B. viridis unigenes is shorter (between 10 and 92%) and likely represents fragments. In contrast, several unigenes are also longer, which may be indicative of insertions, for example by the extension of repetitive regions (Table 2).
Non-anonymous microsatellite markers and sex linkage
For comparative studies of sex chromosomes and autosomes, markers on several autosomal linkage groups, with emphasis on linkage group 2, were developed. In total, twenty-one microsatellite markers were generated from sequences with repetitive patterns found in the transcriptomic dataset (Fig 1, Table 3). Additionally, marker BvIno80b was generated to amplify an indel present in the transcriptome data. All of these microsatellites were polymorphic among B. viridis, B. balearicus, B. siculus and B. variabilis. Markers BvDMRT1, BvVLDLR and BvCHD1 were intron based indel-targeting markers, equally developed from transcriptome data by sequencing introns with primers matching flanking exons.
For markers written in bold, sex linkage was confirmed in green toads (main text for details). Marker names include the gene name abbreviation according to Xenbase. Linkage group size is relative to the proportion of the respective scaffold represented in the X. tropicalis genome v. 7.1 . In green toads, “(Ino80b)” was found to be unlinked to other scaffold 1-homologous markers.
Markers BvCamk4, BvDMRT1, BvCherp, BvHNRNPD and BvVLDLR show a signature of sex-specific transmission of alleles in the offspring of Si337 (mother, B. siculus) and Cr13 (father, B. siculus x B. balearicus). Sex-specific transmission is not perfect since single male specific alleles can be found in females and also single males without specific alleles are present. The marker BvIno80b showed no sex linkage in B. viridis and was therefore considered to be autosomal (S1 Table). For the sex-linked marker C223, allele 163 was perfectly linked to allele 225 of marker BvEll2, and allele 171 linked to allele 162 of the marker BvGar1 (S2 Table).
Cross-amplification trials in representatives from nine systematic anuran families showed variable success for different markers. The number of amplifying markers decreases with increasing evolutionary distance (Fig 2). In B. bufo (23.3 My divergence time to B. viridis) 9/11 markers amplified. In the second bufonid, Rhinella marina (37.3 My), 8/11 markers amplified. The amplification proportion for Dendrobatidae (58.6 My) was at a mean of 4.5/11 markers. For Hylidae and Ranidae (77.9 My) mean amplification success was 5.3/11 markers. In the most distant group consisting of Bombinatoridae and Pipidae (223.2 My) the mean amplification proportion was 3.5/11 and in Pelobates fuscus (Pelobatidae, 196.1 My) 2/11 markers amplified successfully.
The present study aimed at testing whether a single transcriptome of a non-model anuran species may present a reasonable resource for amphibians, where whole genome sequencing remains unaffordable due to large genome size. We have first tested this by retrieving a list of candidate genes, known for their role in sex determination and sex differentiation, and second by the targeted development of non-anonymous microsatellite markers. In terms of completeness, i.e. the presence of at least a fragment of a certain gene, our approach has provided reasonably sufficient data, as we could retrieve 87% of the desired genes. However, and somewhat expected, we face two problems regarding this list: i) deep divergences (ca. 200 My) to the model species may generally lower the blast hit success due to strong sequence divergence, ii) some expected sequences are either completely missing from the transcriptome or have become only available in small portions.
For the development of non-anonymous microsatellite markers, the single transcriptome has been useful. Since these markers are exonic (or UTR-linked), their genomic position can be mapped to the few available and only remotely related reference genomes. In this way, even in non-model species, genomic positions can be inferred based on structural conservation (synteny). Classical short polymorphic tandem-repeated DNA sequences (microsatellites) stem mostly from the non-coding, i.e. >98% of vertebrate genomes . While these multiallelic markers can be easily genotyped, their genomic location usually remains unknown (“anonymous”). Thus, cross-amplification and consequently applicability to diverged lineages and species are often limited. Since exonic regions show a larger degree of sequence conservation, transcriptome-based microsatellites can ensure cross-amplification better than classical non-coding markers [31, 8]. Targeted development of green toad markers homologs on X. tropicalis LG 1, largely homologous to the B. viridis sex chromosome, has been successfully accomplished [23, 15]. For a subset of these markers, sex linkage could be demonstrated in genetic families: 7 out of 8 markers show expected sex-specific transmission in B. viridis (S1 and S2 Tables). Sex-specific transmission is not perfect in the genetic family Si337xCr13 (S1 Table), likely due to meiotic recombination along the B. viridis sex chromosomes, which has been shown in previous studies [28, 23]. Sex linkage of the 7 B. viridis microsatellites corroborates evidence for conserved synteny across the anuran LG 1 for Palearctic green toads. Only marker BvIno80b, located at the distal tip of X. tropicalis LG1 (Fig 1), shows no sex linkage, presumably a result of genome rearrangements.
The new transcriptome-based microsatellite markers also show a high cross-amplification success in several representatives across the anuran phylogeny. In other bufonids, Bufo bufo and R. marina, most markers could be successfully genotyped. Even in Xenopus tropicalis, a species with more than 200 My of divergence to B. viridis, three markers have still amplified successfully (S3 Table). Cross-amplification success inversely correlates with evolutionary distance . Similar results have been shown for anonymous microsatellites in other vertebrate groups such as fish , crocodiles , birds [34, 35] as well as in other amphibians [36, 37]. Cross-amplification success among tree frogs declines by 50% after about 40 My . The ‘half-life’ of our marker set tested for cross-amplification is about 120 My (predicted from regression). Despite the relatively small number of data points to test this relationship, our results suggest that cross amplification trials for transcriptome-based PCR products may be a convenient alternative for developing nuclear markers in anurans.
Our data support the view that single, namely multiple-tissue based transcriptome sequencing is a reliable genomic resource and cost-efficient method for non-model amphibian species with large genome size and despite limitations, should be considered as long as genome sequencing remains unaffordable for most species.
S1 Fig. Frequency length distribution of unigenes in the B. viridis transcriptome.
S2 Fig. Functional GO annotations of B. viridis transcriptome unigenes.
S1 Table. Sex linkage of markers BvCamk4, BvDMRT1, BvCherp, BvHNRNPD, BvIno80b and BvVLDLR.
Genotypes of B. balearicus female (Si337) and F1-male (B. balearicus x B. siculus; Cr13) and their offspring. Phenotypic females are red colored, phenotypic males and alleles, which are expected to show sex-specific transmission, are marked in blue color.
S2 Table. Sex linkage of markers BvEll2 and BvGar1.
Genotypes of Si335 and Si336 and the resulting offspring. Alleles, which show sex-specific transmission, are colored green and orange.
S3 Table. Markers developed for B. viridis that cross-amplified in the tested anuran species.
In all ten examined species at least some of the markers showed bands in the agarose gel. Gradient PCRs were done with all markers to determine the optimal annealing temperature (TA) and the TA range, in which amplification is possible. The approximate fragment length is estimated from the gel pictures.
We thank Alan Brelsford for initial collaboration on RNA extraction; Nicolas Perrin for support; Alexander von Ungern-Sternberg, Panagiotis Kornilios and Petros Lymberakis for help during the field work in Greece (2011); Maria Ogielska, Eva Ringler, Wilbert Bosman, Sylvain Dubey, Wolf-Rüdiger Grosse, and Stefan Lötters for DNA samples. We further thank Katrin Preuss and Michael Monaghan for permission and assistance while using the IGB genotyping facility.
Conceived and designed the experiments: MS. Performed the experiments: JG SR MS. Analyzed the data: JG SR JR CD MS. Contributed reagents/materials/analysis tools: WK CD JG. Wrote the paper: JG MS.
- 1. Ellegren H. Genome sequencing and population genomics in non-model organisms. Trends in Ecology & Evolution. 2014;29(1):51–63.
- 2. Foote AD, Liu Y, Thomas GWC, Vinař T, Alföldi J, Deng J et al. Convergent evolution of the genomes of marine mammals. Nature. 2015;47:272–275.
- 3. Gregory TR. Animal Genome Size Database. 2015; Available: http://www.genomesize.com. Accessed 24 November 2015.
- 4. Hellsten U, Harland RM, Gilchrist MJ, Hendrix D, Jurka J, Kapitonov V et al. The Genome of the Western Clawed Frog Xenopus tropicalis. Science. 2010;328(5978):633–636. pmid:20431018
- 5. Sun Y-B, Xiong Z-J, Xiang X-Y, Liu S-P, Zhou W-W, Tu X-L et al. Whole-genome sequence of the Tibetan frog Nanorana parkeri and the comparative evolution of tetrapod genomes. Proceedings of the National Academy of Sciences. 2015;112(11):E1257–E1262.
- 6. Singhal S. De novo transcriptomic analysis for non-model organisms: an evaluation of methods across a multi-species data set. Molecular Ecology Resources. 2013;13:403–416 pmid:23414390
- 7. Doyle JM, Siegmund G, Ruhl JD, Eo SH, Hale MC, Marra NJ et al. Microsatellite analyses across three diverse vertebrate transcriptomes (Acipenser fulvescens, Ambystoma tigrinum, and Dipodomys spectabilis). Genome. 2013;56(7):407–414. pmid:24099393
- 8. Dufresnes C, Brelsford A, Béziers P, Perrin N. Stronger transferability but lower variability in transcriptomic- than in anonymous microsatellites: evidence from Hylid frogs. Molecular Ecology Resources. 2014;14(4):716–725. pmid:24345298
- 9. Mesak F, Tatarenkov A, Earley R, Avise J. Hundreds of SNPs vs. dozens of SSRs: which dataset better characterizes natural clonal lineages in a self-fertilizing fish? Frontiers in Ecology and Evolution. 2014;2.
- 10. Kitano J, Ross J, Mori S, Kume M, Jones F, Chan Y et al. A role for a neo-sex chromosome in stickleback speciation. Nature. 2009;461(7267):1079–1083. pmid:19783981
- 11. Sankararaman S, Mallick S, Dannemann M, Prüfer K, Kelso J, Pääbo S et al. The genomic landscape of Neanderthal ancestry in present-day humans. Nature. 2014;507(7492):354–357. pmid:24476815
- 12. Stöck M, Moritz C, Hickerson M, Frynta D, Dujsebayeva T, Eremchenko V et al. Evolution of mitochondrial relationships and biogeography of Palearctic green toads (Bufo viridis subgroup) with insights in their genomic plasticity. Molecular Phylogenetics and Evolution. 2006;41(3):663–689. pmid:16919484
- 13. Colliard C, Sicilia A, Turrisi G, Arculeo M, Perrin N, Stöck M. Strong reproductive barriers in a narrow hybrid zone of West-Mediterranean green toads (Bufo viridis subgroup) with Plio-Pleistocene divergence. BMC Evol Biol. 2010;10(1):232.
- 14. Dufresnes C, Bonato L, Novarini N, Betto-Colliard C, Perrin N, Stöck M. Inferring the degree of incipient speciation in secondary contact zones of closely related lineages of Palearctic green toads (Bufo viridis subgroup). Heredity. 2014;113(1):9–20. pmid:24713825
- 15. Tamschick S, Rozenblut-Kościsty B, Bonato L, Dufresnes C, Lymberakis P, Kloas W et al. Sex chromosome conservation, DMRT1 phylogeny and gonad morphology in diploid Palearctic green toads (Bufo viridis subgroup). Cytogenetic and Genome Research. 2015;144(4): 315–324.
- 16. Betto-Colliard C, Sermier R, Litvinchuk S, Perrin N, Stöck M. Origin and genome evolution of polyploid green toads in Central Asia: evidence from microsatellite markers. Heredity. 2014;114(3):300–308. pmid:25370211
- 17. Li R, Zhu H, Ruan J, Qian W, Fang X, Shi Z et al. De novo assembly of human genomes with massively parallel short read sequencing. Genome Research. 2009;20(2):265–272. pmid:20019144
- 18. Altschul SF, Madden TL, Schäffer AA, Zhang J, Zhang Z, Miller W et al. Gapped BLAST and PSI-BLAST: a new generation of protein database search programs. Nucleic Acids Research. 1997;25(17):3389–3402. pmid:9254694
- 19. Conesa A, Götz S, García-Gómez JM, Terol J, Talón M, Robles M. Blast2GO: a universal tool for annotation, visualization and analysis in functional genomics research. Bioinformatics. 2005;21(18):3674–3676. pmid:16081474
- 20. Ye J, Fang L, Hongkun Z, Zhang Y, Chen J, Zengjin Z et al. WEGO: a web tool for plotting GO annotations. Nucleic Acids Research. 2005;34(2):W293–W297.
- 21. James-Zorn C, Ponferrada VG, Burns KA, Fortriede JD, Lotay VS, Liu Y et al. Xenbase; core features, data acquisition and data processing. Genesis, the Journal of Genetics and Development. 2015;53:486–497.
- 22. Miura I. The late replication banding patterns of chromosomes are highly conserved in the genera Rana, Hyla, and Bufo (Amphibia: Anura). Chromosoma. 1995;103(8):567–574. pmid:7621707
- 23. Brelsford A, Stöck M, Betto-Colliard C, Dubey S, Dufresnes C, Jourdan-Pineau H et al. Homologous sex chromosomes in three deeply divergent anuran species. Evolution. 2013;67(8):2434–2440. pmid:23888863
- 24. Legendre M, Pochet N, Pak T, Verstrepen K. Sequence-based estimation of minisatellite and microsatellite repeat variability. Genome Research. 2007;17(12):1787–1796. pmid:17978285
- 25. Cunningham F, Amode M, Barrell D, Beal K, Billis K, Brent S et al. Ensembl 2015. Nucleic Acids Research. 2014;43(D1):D662–D669.
- 26. Untergasser A, Cutcutache I, Koressaar T, Ye J, Faircloth B, Remm M et al. Primer3—new capabilities and interfaces. Nucleic Acids Research. 2012;40(15):e115–e115. pmid:22730293
- 27. Stöck M, Croll D, Dumas Z, Biollay S, Wang J, Perrin N. A cryptic heterogametic transition revealed by sex-linked DNA markers in Palearctic green toads. Journal of Evolutionary Biology. 2011;24(5):1064–1070. pmid:21338434
- 28. Stöck M, Savary R, Betto-Colliard C, Biollay S, Jourdan-Pineau H, Perrin N. Low rates of X-Y recombination, not turnovers, account for homomorphic sex chromosomes in several diploid species of Palearctic green toads (Bufo viridis subgroup). Journal of Evolutionary Biology. 2013;26(3):674–682. pmid:23316809
- 29. R Development Core Team. R: A Language and Environment for statistical computing. Vienna, Austria; 2015. Available: http://www.R-project.org. Accessed 7 September 2015.
- 30. Gregory RT. Synergy between sequence and size in Large-scale genomics. Nat Rev Genet. 2005;6(9):699–708. pmid:16151375
- 31. Dawson DA, Ball AD, Spurgin LG, Martín-Gálvez D, Stewart IR, Horsburgh GJ et al. High-utility conserved avian microsatellite markers enable parentage and population studies across a wide range of species. BMC Genomics. 2013;14(1):176.
- 32. Carreras-Carbonell J, Macpherson E, Pascual M. Utility of pairwise mtDNA genetic distances for predicting cross-species microsatellite amplification and polymorphism success in fishes. Conservation Genetics. 2007;9(1):181–190.
- 33. Glenn T, Stephan W, Dessauer H, Braun M. Allelic diversity in alligator microsatellite loci is negatively correlated with GC content of flanking sequences and evolutionary conservation of PCR amplifiability. Molecular Biology and Evolution. 1996;13(8):1151–1154. pmid:8865669
- 34. Primmer C, Moeller A, Ellegren H. A wide-range survey of cross-species microsatellite amplification in birds. Molecular Ecology. 1996;5(3):365–378. pmid:8688957
- 35. Primmer CN, Painter JN, T. Koskinen MT, Palo JU, Merilä J. Factors affecting avian cross-species microsatellite amplification. Journal of Avian Biology. 2005;36(4):348–360.
- 36. Hendrix R, Hauswaldt S, Veith M, Steinfartz S. Strong correlation between cross-amplification success and genetic distance across all members of ‘True Salamanders’ (Amphibia: Salamandridae) revealed by Salamandra salamandra-specific microsatellite loci. Molecular Ecology Resources. 2010;10(6):1038–1047. pmid:21565114
- 37. Nair A, Gopalan S, George S, Kumar K, Merilä J. Cross-species testing and utility of microsatellite loci in Indirana frogs. BMC Research Notes. 2012;5(1):389.