|Home | About | Journals | Submit | Contact Us | Français|
For many years, parasitic B chromosomes have been considered genetically inert elements. Here we show the presence of ten protein-coding genes in the B chromosome of the grasshopper Eyprepocnemis plorans. Four of these genes (CIP2A, GTPB6, KIF20A, and MTG1) were complete in the B chromosome whereas the six remaining (CKAP2, CAP-G, HYI, MYCB2, SLIT and TOP2A) were truncated. Five of these genes (CIP2A, CKAP2, CAP-G, KIF20A, and MYCB2) were significantly up-regulated in B-carrying individuals, as expected if they were actively transcribed from the B chromosome. This conclusion is supported by three truncated genes (CKAP2, CAP-G and MYCB2) which showed up-regulation only in the regions being present in the B chromosome. Our results indicate that B chromosomes are not so silenced as was hitherto believed. Interestingly, the five active genes in the B chromosome code for functions related with cell division, which is the main arena where B chromosome destiny is played. This suggests that B chromosome evolutionary success can lie on its gene content.
Many supernumerary (B) chromosomes are rich in repetitive satellite and ribosomal DNA sequences, and their unusual meiotic dynamics and dispensable nature makes them an easy target for the integration and expansion of transposable elements (TEs)1,2. Many other kinds of DNA sequences could be interspersed among these repeats. This was first shown in the B chromosomes of rye (Secale cereale), which bear specific repeats and insertions of organellar DNA as well as gene-derived sequences showing fragmentation and pseudogenization3, including at least one functional gene4.
Although the high enrichment of repetitive DNA in B chromosomes hindered the detection of protein-coding genes in them, things have changed in the last decade by the discovery of proto-oncogenes and tumor-suppressor genes in the B chromosomes of several canid species5,6, H3 and H4 histone genes in those of the migratory locust7, and other protein-coding genes in the B chromosomes of a cichlid fish8 and two cervid species9,10. In addition, Valente et al. analyzed the gene content of B chromosomes by comparing Illumina sequences from 0B and 2B genomes in the cichlid fish Astatotilapia latifasciata, with subsequent confirmation by quantitative PCR and FISH mapping, complemented by Roche 454 sequencing of a microdissected B chromosome. They mapped those sequences to the scaffolds of the genome of the cichlid Metriaclima zebra, and detected blocks where the B+/B− coverage was higher than the average calculated for scaffolds not located in the B. Those blocks with high coverage in the B+ library where further annotated with the M. zebra genome. Among them, they found more than 5,000 sequences putatively identified as genes, besides repeats and transposable elements. Most of the genes found in the B chromosome were fragmented, but a few of them were complete and associated with functions such as microtubule organization, kinetochore structure, recombination and progression through the cell cycle, which may be involved in the transmission and maintenance of the parasitic chromosome11.
The general belief that B chromosomes are genetically inactive was enforced by experiments using tritiated uridine in the grasshoppers Myrmeleotettix maculatus and Chorthippus paralelus12, and in the rodent Apodemus peninsulae13. Nevertheless, gene expression in B chromosomes is probably behind the remarkable effects reported in some cases, such as the fungus Nectria haematococca, whose B chromosome carries a gene which confers resistance to pisatin, an antibiotic produced by the pea host plant14, or the paternal sex ratio (PSR) chromosome of the parasitic wasp Nasonia vitripennis, which causes the conversion of diploid zygotes (destined to be females) to haploid males15. More recently, it has been shown that B chromosomes influence sex determination in cichlid fishes8. Consistently, gene expression has recently been found in B chromosomes of several species. For instance, the presence of rRNA transcripts specifically coming from B chromosomes has been shown in the plant Crepis capillaris16, the parasitic wasp Trichogramma kaykai17 and the grasshopper Eyprepocnemis plorans18. Also, Carchilan et al. showed, in rye, the presence of B-specific transcribed DNA sequences belonging to high-copy number families with similarity to mobile elements19, while Zhou et al. characterized a B chromosome linked scaffold that contains an actively transcribed unit20, and Trifonov et al.reported the transcription of protein coding genes in Capreolus pygargus9. Recently, it has been reported that a repetitive element enriched in a B chromosome may code for a long non-coding RNA21 Thus, it has been suggested that B chromosome content might influence the expression of genes located in the standard A genome19,21,22,23. Indeed, genomic and transcriptomic analyses have revealed the presence of pseudogenic and functional copies of the Argonaute-like AGO4B gene on rye B chromosomes4.
The B chromosome system of E. plorans is very widespread and highly polymorphic, with Bs being present in almost all populations from the circum-Mediterranean region24. The presence of a same type of B in populations from Spain, Morocco, Tunisia and Sicilia suggests a recent invasion into these areas25. The high success of these B chromosomes, which are present in almost all populations hitherto analyzed, except those in the headwaters area of the Segura River basin in Spain26, has arisen from the transmission advantage (drive) they show during female meiosis27. This drive is suppressed by the A chromosomes28,29 as a consequence of the arms race between A and B chromosomes predicted by the near-neutral model of B chromosome evolution30. Neutralized B chromosomes (e.g. B2) can undergo chromosomal rearrangements (see examples in López-León et al.31), some of which might give rise to a new B-variant being able to drive (e.g. B24 in the Torrox population) thus replacing the neutralized variant27,32. Logically, this polymorphism regeneration prolongs very much the lifespan of the B chromosome polymorphism.
B chromosomes of E. plorans are able to transcribe their rDNA and organize a nucleolus18, although this occurs only in a minority of males from most populations33, and the rRNA contribution by the B to total rRNA is insignificant compared to that from A chromosomes34, suggesting that B chromosomes in this species are highly repressed. Here we analyze the possible presence of protein-coding genes in the B chromosome of this species by means of NGS analysis of 0B and 4B male genomes and their mapping against the coding sequence (CDS) regions of a de novo assembled transcriptome built with all the reads obtained from 0B and 1B female RNAs. This approach has revealed the presence of ten protein-coding genes, five of which are actively transcribed in males and females.
Clustering and identification of potential CDSs in the de novo assembled E. plorans transcriptome yielded 13,190 sequences that were used as reference for mapping and comparative coverage analysis in 0B and 4B gDNA libraries (E. plorans transcriptome assembled de novo can be accessed in Figshare at https://dx.doi.org/10.6084/m9.figshare.3408580.v3).
The mapping of the Illumina reads from the 0B and 4B genomes on the coding sequences (CDS) of the de novo transcriptome revealed 2,592 CDSs with 40 or more mapped reads (considering both libraries). Graphical representation of the 0B and 4B libraries showed the presence of some CDSs being over-represented in the 4B library (Fig. 1). Remarkably, 29 CDSs showed a log2 4B/0B quotient >1.58, i.e. the expected value if each B chromosome carried one copy of the CDS (see materials and methods). Annotation revealed that 13 of these CDSs were orthologous to 8 different protein-coding genes in the L. migratoria genome35 (Table 1): CIP2A (CIP2A protein), CKAP2 (Cytoskeleton-associated protein 2), CAP-G (Condensin I complex subunit G), GTPB6 (GTP-binding protein 6), KIF20A (Kinesin-like protein KIF20A), MTG1 (Mitochondrial GTPase 1), MYCB2 (E3 ubiquitin-protein ligase MYCBP2), and TOP2A (DNA topoisomerase 2-alpha). In adition, for qPCR analysis, two other annotated CDSs were selected (HYI (Hydroxypiruvate isomerase) and SLIT (SLIT protein)) which, in a preliminary analysis, showed higher abundance in the 4B genome compared to 0B. The sequences of these ten transcripts can be found in GenBank under accession numbers KX034164 to KX034172 and KY211688 (Table 2).
According to the coverage pattern observed in 0B and 4B genomes, full length CDSs were found in the 4B genome for four genes: CIP2A, GTPB6, KIF20A and MTG1, suggesting that these genes might be complete on the B chromosome. As shown in Fig. 2A and Supplementary Figs S1A, S2A and S3A, coverage for these genes in the gDNA 4B library was uniformly high along all CDS length. The six remaining genes (MYCB2, CAP-G, CKAP2, HYI, SLIT and TOP2A), however, appeared to be incomplete on the B chromosome. MYCB2 was clearly truncated (Fig. 3A), showing only the last 5,764 nucleotides of the 3′ end out of the 14,434 nucleotides reported for the orthologous gene in L. migratoria. In CAP-G, the last five exons (exons 20–24) of the CDS reported for the L. migratoria genome show low coverage in the E. plorans 4B genome (Supplementary Fig. S4A). In CKAP2, the 5′ UTR and 396 nucleotides of the 5′ end of the CDS seem to be missing (Supplementary Fig. S5A). For HYI, we only observed 85 nucleotides in the 3′ end of the CDS plus the 3′ UTR, but this gene actually showed very low coverage in both gDNA libraries, and its integrity was difficult to assess (Supplementary Fig. S6A). In the case of the SLIT gene, only the last two exons of the 5′ end were in the B chromosome, out of the 30 exons reported in L. migratoria (Supplementary Fig. S7A). Finally, TOP2A coverage in the 4B library was low from nucleotide 3,465 to the 3′ end of the transcript, suggesting that this part is not present in the B chromosome copies (Supplementary Fig. S8A).
On the basis of mean abundances per nucleotide position in 0B and 4B libraries (A0B and A4B, respectively) inferred from mapping Illumina gDNA reads onto transcriptome CDS regions, and assuming that these ten genes are single-copy in the A chromosome set, we estimated the number of copies in the B-carrying genome (N4B) and also per B chromosome (NB). This suggested the presence of two or more copies for all ten genes in the B chromosome, with NB ranging from 2 to 17 (Table 2).
qPCR experiments on gDNA from males carrying 0–3 B chromosomes showed that genomic abundance for these ten genes increased linearly with the number of B chromosomes (Figs 2B and and3B,3B, Supplementary Table S1 and Supplementary Figs S1B–S7B), thus giving high support to the NGS results. Remarkably, in the six truncated genes (MYCB2, CAP-G, CKAP2, HYI, SLIT and TOP2A) this linear relationship was observed only in the region showing high coverage in the gDNA 4B library, implying their location in the B chromosome, while no relationship with B number was observed for the low coverage region thus supporting its absence on the B chromosome and the existence of fragmented B chromosome gene copies (see Fig. 3B and Supplementary Figs S4B–S8B).
The analysis of differential gene expression between B-carrying and B-lacking individuals, by means of qPCR, revealed that five out of the ten genes located on the B chromosome (CIP2A, CKAP2, CAP-G, KIF20A, and MYCB2) showed significant up-regulation in B-carrying males (all genes) and females (all except KIF20A) (Supplementary Table S2), suggesting that some of the B-located gene copies are transcribed. Remarkably, three of these genes (MYCB2, CAP-G and CKAP2) are truncated on the B chromosome and showed differential expression only for the gene regions contained in the B chromosome but not for missing regions (see Figs 3C, S4C and S5C, and Supplementary Table S2). This strongly supports that the up-regulation of these genes is due to the activity of the B chromosome copies and not simply to up-regulation of the A chromosome gene copies.
For CIP2A (Fig. 2C) and KIF20A (only in males, Supplementary Fig. S2C) genes, expression level increased with B chromosome number, and a similar dosage effect was observed for MYCB2 (Fig. 3C), CAP-G (Supplementary Fig. S4C) and CKAP2 (Supplementary Fig. S5C) in the case of gene regions being present in the B chromosome, whereas, in TOP2A, this association was only marginally significant (Supplementary Fig. S8C). No significant differential expression was found for the gene regions being missing in the B chromosome for MYCB2 (Fig. 3C), CAP-G (Supplementary Fig. S4C), CKAP2 (Supplementary Fig. S5C) and TOP2A (Supplementary Fig. S8C), or for the GTPB6 (Supplementary Fig. S1C), MTG1 (Supplementary Fig. S3C), HYI (Supplementary Fig. S6C) and SLIT (Supplementary Fig. S7C) genes. Taken together, these results reinforce the conclusion that about half of the B chromosome genes identified here are actively transcribed.
Gene Ontology (GO)36 analysis for these ten genes revealed potential implication in biological processes likely profitable for a parasitic B chromosome, such as the regulation of mitotic cell cycle (KIF20A, CAP-G, and CKAP2), DNA replication and regulation of transcription (CKAP2 and MYCB2), apoptotic processes and regulation of cell death (CKAP2), chromosome condensation and organization (CAP-G and TOP2A), chromosome segregation (CAP-G and TOP2A), cell-cell signaling and cellular response to stimulus (SLIT), and reproductive structure development (SLIT) (see Supplementary Dataset 1). The EuKaryotic Orthologous Groups (KOG)37 classification of these ten genes also gave interesting indications of their potential functions (Table 3), some of which being highly valuable for the advantageous transmission of this parasitic chromosome. For instance, CIP2A and KIF20A have functions related with cytoskeleton and thus microtubule dynamics, CAP-G and TOP2A are related with chromosome condensation and chromatin structure and dynamics, and thus with cell cycle control. The two former genes appear to be complete and active in the B chromosome, but the two latter are truncated thus probably rendering non-translated or inactive transcripts.
As intranuclear parasites, B chromosomes mimic A chromosomes in many respects, for example the structure and organization of the DNA sequences contained in them, although they are usually heterochromatic and, as such, assumed to be genetically inert elements (for review, see Camacho2).
Recently, transcription of a protein-coding gene on B chromosomes of the Siberian roe deer (Capreolus pygargus) has been shown9, while Banaei-Moghaddam et al. used NGS to demonstrate that about 15% of the pseudogene-like fragments on B chromosomes are transcribed following a pattern related to genotype and tissue type, with some of them apparently playing a role in trans-regulation of genes located in the A chromosomes22. Likewise, Valente et al. analyzed transcriptome sequences from the cichlid fish, Pundamilia nyererei, and some of them showed high sequence similarity with the B-encoded variants for the Separin, TUBB1 and KIF11 genes found in Astatotilapia latifasciata, thus suggesting that P. nyererei might have B chromosomes expressing these genes11. These findings clearly contradict the “B genetic inertness” hypothesis, although whether B chromosomes express truly functional genes (i.e. generate proteins) or regulatory factors (i.e. small RNAs) remains to be tested. Recently, Ma et al. have shown that rye B chromosomes carry active Argonaute-like genes showing in vitro slicer activity, thus opening the interesting prospect that B chromosomes may carry functional genes influencing other genes’ expression or cellular processes4. However, the only B chromosome genes which have been shown to yield functional transcripts in vivo are those for rRNA in the grasshopper E. plorans, as they give rise to the expected phenotype, i.e. a nucleolus18.
Here we show that B chromosomes in E. plorans contain at least ten protein-coding genes, with full CDS regions in four of them. The qPCR validation of two genes failing to meet the a priori selection criteria of the NGS analysis (i.e. HYI and SLIT) demonstrated a positive correlation with number of B chromosomes, indicating that the NGS selection criteria are actually conservative and that these B chromosomes most likely carry other undetected genes. Remarkably, five of these ten genes are actively transcribed in E. plorans. Many of the B-derived transcripts might be functionless because the gene copies on the B chromosome are incomplete, so that their translation would yield anomalous polypeptides which could potentially pose metabolic stress on cells. Alternatively, these gene fragments could interfere A chromosome gene expression by competitively binding transcription factors38,39,40. However, we cannot rule out that the transcripts from some B-located genes, being apparently complete, can be functional, as previously observed for 45S rRNA transcripts18. Of course, the possibility that a B chromosome can contribute gene products which are useful for its own survival (e.g. through cell division) is a new and interesting prospect in B chromosome research.
Three genes which are truncated on the B chromosome (CKAP2, CAP-G and MYCB2) show up-regulation only for the region being present in the B chromosome, indicating that gene copies located on the B chromosome are transcribed, although our data cannot differentiate this from a more complex transcriptional regulatory pathway involving A and B copies. CKAP2 codes for a cytoskeleton-associated protein which localizes to spindle poles and microtubules from prophase to anaphase41, and seems to play an important role in chromosome segregation and stability42,43. CAP-G codes for a subunit of the Condensin I chromosome condensation complex, subunit G44, whereas MYCB2 encodes a component protein of the anaphase promoting complex (APC) governing the exit from mitosis45. If these transcripts were translated, they would presumably yield non functional truncated polypeptides, especially MYCB2, where more than half of the CDS is missing in the B chromosome. It is however tempting to speculate whether the strong functional relationship between CAP-G and TOP2A in sister chromatid resolution46 and chromosome condensation47 might have played a role in the invasion of the E. plorans genome by this B chromosome, in the event that these genes were ever complete and functional in it.
It is also conceivable that, as suggested by Banaei-Moghaddam et al., these gene fragments present in the B could act as trans modulators, affecting the activity of its counterparts located in the A genome22. A possible example of this could be the down-regulation shown by the GTPB6 gene in the 1B RNA library (see Supplementary Fig. S1A), meaning that it would be repressed in presence of the B chromosome, and a similar trend was observed in qPCR experiments on ovary (Supplementary Fig. S1C), although it was not significant (Supplementary Table S2).
Remarkably, the two remaining up-regulated protein-coding genes (CIP2A and KIF20A), which were complete in the B chromosome, coded for potentially interesting functions for a parasitic chromosome. CIP2A codes for an oncoprotein that inhibits protein phosphatase 2A (PP2A), promoting anchorage-independent cell growth and tumor formation, and its overexpression causes premature chromosome segregation and aneuploidy48. Bearing in mind that B chromosomes most likely originate as a kind of aneuploidy2,49, it is conceivable that the excess of CIP2A gene products, provided by transcription from the B chromosome copies, might be advantageous for B chromosome maintenance. Likewise, KIF20A codes for a mitotic kinesin required for chromosomal passenger complex (CPC) transport during cytokinesis50 and for appropriate assembly of microtubules at anaphase and metaphase-anaphase transition51. In Xenopus, Takemoto et al. showed that PP2A plays a role in the recruitment and targeting of Condensin II and kinesin protein KIF4a to chromosomes during mitosis, and PP2A inhibition causes Condensin II and KIF4a dissociation from assembled chromosomes52. In E. plorans, B chromosomes carrying active CIP2A and KIF20A genes could potentially influence the course of cell division for their own benefit, thus revealing their true parasitic nature. In rye, the presence of repetitive DNA sequences in the short arm of the B chromosome promotes mitotic nondisjunction which is the basis for its drive mechanism53. In E. plorans, B chromosome drive takes place during female meiosis27,28, and the possibility of manipulating it through gene expression might be the basis for the high success of B chromosomes in this species, as they are present in almost all natural populations hitherto analyzed24.
Taken together, our results show, for the first time, that the secret for B chromosome success may lie in its gene content, as suggested by the active transcription of the complete CDS of CIP2A and KIF20A and the fragments of CKAP2, CAP-G and MYCB2, all being genes with functions related with cell division. Interestingly, the presence of this kind of active genes in E. plorans B chromosomes opens new avenues to investigate why neutralized B variants are replaced for newly driving ones, a fact reported several times in this species27,30,32. The possibility that a chromosomal rearrangement in a neutralized B chromosome can elicit position effects changing the expression state of B chromosome genes with functions related with cell division, can now be investigated by comparing gene expression levels for B-genes between different B-variants.
E. plorans individuals were collected in Torrox (Málaga) (Table 4), a population where the prevalent B chromosome variant is B2425. Males were anaesthetized before dissecting out testes, one of which was fixed in 3:1 ethanol-acetic acid for cytological analysis, while the other testis and body remains were frozen in liquid nitrogen for nucleic acid extraction. The number of B chromosomes in males was determined by C-banding of testicular follicles. In the case of the two females used for transcriptome analysis, the number of B chromosomes was determined in interphase hemolymph nuclei54. The full bodies of the two females selected for transcriptome analysis (one 0B and one with 1B) were frozen in liquid nitrogen. The remaining females were anaesthetized before dissecting out the ovaries. A few ovarioles were incubated in 2% colchicine in isotonic insect saline solution for 2h, and then fixed in 3:1 ethanol-acetic acid for cytological analysis. The remaining ovarioles were frozen in liquid nitrogen for gene expression analysis. Body remains were frozen in liquid nitrogen for later nucleic acid extraction. In these females, the number of B chromosomes was determined by C-banding on the colchicine-treated ovarioles. Additionally, B chromosome presence/absence was corroborated in both sexes by PCR amplification of the B-specific SCAR marker, described by Muñoz-Pajares et al.55, on genomic DNA.
Genomic DNA (gDNA) was extracted from hind legs using the GenElute Mammalian Genomic DNA Miniprep kit (Sigma). Quality was checked by TBE-agarose gel electrophoresis and also by measuring 260/280 and 260/230 ratios with an Infinite M200 Pro NanoQuant (Tecan). Total RNA extractions from frozen bodies were performed using a Real Total RNA Spin Plus kit (Durviz), whereas RNA extractions from gonads were done using the RNeasy Lipid Tissue Mini Kit (Qiagen), following manufacturer’s recommendations. In both protocols, we carried out a DNAse treatment on the column membrane (20 units during 30 minutes incubation, DNAse Amplification Grade I, Sigma), to avoid gDNA contamination, which was validated by PCR amplification of rDNA or histone genes in the extracted RNA and subsequent visualization on an agarose gel. In body samples, a second DNAse treatment was performed after the extractions, using the REALSTAR kit (Durviz). Quality and quantity of RNA was assessed with a Tecan’s Infinite 200 NanoQuant spectrophotometer and in a denaturing MOPS-agarose gel to ensure the absence of RNA degradation.
Total RNA was extracted from each of two females, one lacking B chromosomes (0B) and the other carrying 1B, whereas gDNA was collected from two males (0B and 4B; Table 4). Each of the four libraries (gDNA 0B, gDNA 4B, RNA 0B, RNA 1B) was sequenced on an Illumina Hiseq2000 platform, each yielding about 5Gb of paired-end reads (2×101 nucleotides). Illumina sequences are available in NCBI SRA database under accession numbers SRR2970625 (gDNA 0B), SRR2970627 (gDNA 4B), SRR2969416 (RNA 0B) and SRR2969417 (RNA 1B).
We used an E. plorans de novo transcriptome35 asembled using Trinity56, as reference for read mapping. We reduced redundancies with CD-HIT-EST57 with local alignment and greedy algorithm, and grouped those sequences showing 80% or higher similarity in at least 80% of length (options -M 0 -aS 0.8 -c 0.8 -G 0 -g 1). Potential CDSs were predicted with Transdecoder56, considering open reading frames (ORFs) longer than 300 nucleotides. Functional annotation of CDSs was performed with Trinotate56 against the Uniprot database58, and the identification of transposable elements (TEs) within the CDS was performed with RepeatMasker59 in a database including TEs described in Locusta migratoria (data obtained from RepBase60).
To search for protein-coding genes residing in the B chromosome, we performed the following analysis. Against the de novo transcriptome, we mapped: 1) the reads obtained from the 0B and 4B genomes (gDNA 0B and gDNA 4B libraries), and 2) those obtained from RNA sequencing in 0B and 1B females (RNA 0B and RNA 1B libraries). We mapped the reads using SSAHA261 with a minimum alignment score of 40 and 80% minimum identity. We used a custom script (https://github.com/fjruizruano/ngs-protocols/blob/master/count_reads_bam.py) to count the number of mapped reads as a measure of abundance (see a graphical summary of analysis workflow in Supplementary Fig. S9).
We selected coding sequences (CDS) putatively being located in the B chromosome on the basis of the two following criteria: 1) the sum of mapped reads (adding those from 0B and 4B gDNA libraries) should be 40 or higher, and 2) log2 of the quotient between the number of mapped reads in the 4B and 0B gDNA libraries (4B/0B) was equal to or higher than 1.58. This figure was inferred by assuming that a single-copy gene would have two copies in a diploid 0B genome, whereas, if each B chromosome would carry one copy then the 4B genome would carry six copies, i.e. three times more copies than the 0B one, so that log2 (3)=1.58.
We analyzed the integrity and structure of the B-located genes using a transcriptome assembly from 12 RNA-Seq libraries of Locusta migratoria (Ruiz-Ruano et al., personal communication) and the L. migratoria genome assembled by Wang et al. (accession number AVCP000000000)35. We searched for homologous sequences in the L. migratoria transcriptome with BLASTN62. Using the sequence with the lowest E-value as reference for a second BLASTN62, we searched for homologous sequences in the L. migratoria genome. We aligned our transcripts from E. plorans to the selected genomic sequences with the exonerate software63 to search for exon junction sites. If an E. plorans transcriptome sequence was incomplete with respect to the L. migratoria one, we used the homologous contig of L. migratoria transcriptome as reference for further assembling of the E. plorans contigs, to full-length E. plorans transcripts wherever possible. Using them as reference, we performed a new SSAHA262 mapping to test the completeness of the CDSs of these genes in the B chromosome. We thus analyzed abundance per nucleotide position for each CDS in the 0B and 4B genomes using a custom script (https://github.com/fjruizruano/ngs-protocols/blob/master/bam_coverage_join.py), and calculated it as the proportion of reads mapped at each position, in respect to total number of reads in the corresponding library. This allowed detecting whether a CDS was completely covered by the B-carrying gDNA reads, thus implying its full length presence in the B chromosome. Alternatively, a sharp decrease in nucleotide coverage along CDS length indicated truncation for the corresponding gene in the B chromosome. For full CDSs, we calculated the mean abundance for its whole length in 0B and 4B gDNA libraries. In the case of truncated CDSs, we calculated mean abundance for the highly covered region.
Mean abundance for each CDS (named A0B and A4B in 0B and 4B males, respectively) was used to estimate the number of copies for the corresponding gene in the B-carrying genome, assuming the presence of one copy per A genome set. For this purpose, we first calculated genome size of 0B and 4B males. According to Ruiz-Ruano et al., the E. plorans genome is 1.78 times larger than that of Locusta migratoria64. On this basis these authors got estimates of DNA content of A and B chromosomes in E. plorans, using previous estimates of C.value in L. migratoria (5.89pg=5.76Gb). However, Wang et al. later showed that the sequenced genome of this latter species is actually larger (6.3Gb)35, for which reason we have recalculated, in E. plorans, the DNA amount in the haploid A chromosome set (C-value), and those in the X and B24 chromosomes, being 11.214Gb, 1.352Gb and 0.684Gb, respectively. Bearing in mind that males of this species are X0, we calculated genome size in the 0B and 4B males (G0B=20.58Gb and G4B=23.26Gb, respectively).
The number of gene copies in the B-carrying genome (N4B) was then calculated by the following equation:
where 2 means assuming the presence of one gene copy per A chromosome set. The number of gene copies per B chromosome (NB) was then calculated as:
where 4 is the number of B chromosomes in the B-carrying male.
Gene function classifications were performed according to two standardized methods: Gene Ontology (GO)36 and Eukaryotic Orthologous Groups (KOG)37. GO assignments to predicted proteins were performed with Blast2GO65, and KOG classification was performed with the WebMGA software66, searching the KOG database of NCBI.
Quantification of relative copy number for the B chromosome genes was performed in 16 males from Torrox carrying 0–3 B chromosomes (Table 4). Transcription of B-located genes was analyzed in 23 males and 21 females from Torrox (Table 4), separately in the gonads and the rest of the body. cDNA synthesis was performed by retro-transcription of 100ng per sample of total RNA using a combination of random and oligo dT hexamers (PrimeScript RT reagent Kit, Perfect Real Time, Takara). The cDNA obtained was diluted in RNase-DNase free water for a 1:10 working solution.
Quantitative PCR was performed on a Chromo 4 Real Time PCR thermocycler (Biorad). Primers were designed with Primer367 (see sequences in Table 5). Each reaction mixture contained 5μl of gDNA at 5ng/μl (25ng gDNA per reaction) or 5μl of cDNA working solution obtained as described above, 5μl of SensiMix SYBR Kit (Bioline) and 2.5μl of each 2.5μM primer. Reactions were carried out in duplicate and the coefficient of variation was lower than 8% in all cases. We estimated the amplification efficiency (E) of each primer pair in gDNA or cDNA experiments by means of a standard curve performed on a 10-fold dilution series of E. plorans gDNA or cDNA mixture from several individuals with different numbers of B chromosomes, which was also used as an external calibrator. Then the relative abundance of each gene in 0B, 1B, 2B and 3B genomes was calculated according to RQ=ECtC−CtS. where RQ=Relative quantity, E=Amplification efficiency (fold increase per cycle), CtC=Ct value of the calibrator sample and CtS=Ct value of each sample.
RQs of the expression analysis were calculated according to the same formula, but RQ values were normalized by the geometrical average of several housekeeping genes, i.e. Ribosomal Protein 49 (RP49), Actin 5C (ACT), Armadillo (ARM), and α-tubulin 1A (TUB), selected using GeNorm68. We used RP49+ACT+ARM for female bodies, ACT+ARM for ovaries, ACT+TUB for male bodies and ACT+RP49 for testis. Amplification, sequencing, efficiency and stability analysis of these housekeeping genes in E. plorans was previously performed in Navarro-Domínguez et al.69
For qPCR validation of gene presence in the B chromosome, we should expect that those genes actually residing in the B chromosome would show RQ values on gDNA linearly increasing with the number of B chromosomes. This relationship was tested by the Spearman’s rank correlation test. Differential gene expression was tested by means of Kruskal-Wallis tests comparing individuals with different number of B chromosomes. In all cases, the sequential Bonferroni test was applied to minimize type I errors.
How to cite this article: Navarro-Domínguez, B. et al. Protein-coding genes in B chromosomes of the grasshopper Eyprepocnemis plorans. Sci. Rep. 7, 45200; doi: 10.1038/srep45200 (2017).
Publisher's note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
This work was supported by the Spanish Ministerio de Economía y Competitividad (grant numbers CGL2009-11917, CGL2015-70750-P) and Plan Andaluz de Investigación (grant number CVI-6649), and was partially performed by FEDER funds.
The authors declare no competing financial interests.
Author Contributions B.N.-D., F.J.R.-R., J.C., M.D.L.-L. and J.P.M.C. designed the experiments and obtained the materials for molecular and cytological analyses. B.N.-D. and F.J.R.-R. developed the bioinformatic protocol to find protein-coding genes in B chromosomes. B.N.-D. and F.J.R.-R. performed the bioinformatics analyses. B.N.-D. performed nucleic acid extractions and qPCR. M.D.L.-L. and J.C. determined the number of B chromosomes. B.N.-D. and J.P.M.C. performed statistical analyses. All authors participated in the analysis and discussion of results and paper writing.