- Research article
- Open Access
Signatures of host specialization and a recent transposable element burst in the dynamic one-speed genome of the fungal barley powdery mildew pathogen
BMC Genomics volume 19, Article number: 381 (2018)
Powdery mildews are biotrophic pathogenic fungi infecting a number of economically important plants. The grass powdery mildew, Blumeria graminis, has become a model organism to study host specialization of obligate biotrophic fungal pathogens. We resolved the large-scale genomic architecture of B. graminis forma specialis hordei (Bgh) to explore the potential influence of its genome organization on the co-evolutionary process with its host plant, barley (Hordeum vulgare).
The near-chromosome level assemblies of the Bgh reference isolate DH14 and one of the most diversified isolates, RACE1, enabled a comparative analysis of these haploid genomes, which are highly enriched with transposable elements (TEs). We found largely retained genome synteny and gene repertoires, yet detected copy number variation (CNV) of secretion signal peptide-containing protein-coding genes (SPs) and locally disrupted synteny blocks. Genes coding for sequence-related SPs are often locally clustered, but neither the SPs nor the TEs reside preferentially in genomic regions with unique features. Extended comparative analysis with different host-specific B. graminis formae speciales revealed the existence of a core suite of SPs, but also isolate-specific SP sets as well as congruence of SP CNV and phylogenetic relationship. We further detected evidence for a recent, lineage-specific expansion of TEs in the Bgh genome.
The characteristics of the Bgh genome (largely retained synteny, CNV of SP genes, recently proliferated TEs and a lack of significant compartmentalization) are consistent with a “one-speed” genome that differs in its architecture and (co-)evolutionary pattern from the “two-speed” genomes reported for several other filamentous phytopathogens.
Powdery mildews (Ascomycota, Erysiphales) are ubiquitous fungal plant pathogens in temperate regions of the world . They thrive on the basis of an obligate biotrophic lifestyle, i.e., by retrieving nutrients from living plant cells for fungal growth and reproduction, and have been extensively studied regarding molecular and genetic interactions with both host  and non-host plants . Despite advances in the deployment of durable resistance , powdery mildews remain a constant threat for economically important crops as they rapidly evade selection pressure resulting from fungicide application [5, 6] and resistance (R)-gene mediated immunity . The barley powdery mildew pathogen, Blumeria graminis f.sp. hordei (Bgh), is a member of the species Blumeria graminis that is specialized on its host plant, barley (Hordeum vulgare). There are various specialized forms (formae speciales) of B. graminis, where each forma specialis (f.sp.) is capable of infecting the respective host plant species belonging to the grasses (Poaceae) family, including cereals . Within each forma specialis, numerous isolates (strains) can be differentiated, primarily based on their respective virulence/avirulence phenotypes on particular genotypes of the host population . Meanwhile, B. graminis has become a model organism to study host specialization of obligate biotrophic fungal pathogens.
With the dawn of next-generation sequencing, several studies provided initial insights in the haploid genomes of powdery mildews and the molecular basis of their obligate biotrophic lifestyle. Indeed, the first genomic studies, coupled with other “omics” approaches , showed that powdery mildews have experienced the loss of several, otherwise widely conserved Ascomycete genes with functions related to carbohydrate degradation, primary and secondary metabolism [11, 12], which could explain their strict dependence on live plant tissue. On the other hand, these genomes harbor an abundance of candidate secreted effector protein (CSEP)-coding genes, which were deemed to be crucial for successful pathogenesis [12, 13]. Isolate-specific variants of these powdery mildew CSEPs are recognized by matching intracellular immune receptors, encoded by barley or wheat R genes, which are present only in particular genotypes of these cereal hosts [9, 14, 15]. This demonstrates that at least these CSEPs are targets of the plant immune system and indicates co-evolutionary dynamics underlying interactions between the pathogen and cereal hosts at the population level. Genome sequencing of members of the cereal powdery mildew pathogen, B. graminis, led to the understanding that host specialization can occur by hybridization between two reproductively isolated formae speciales that multiply on different host species  and, possibly, also by “host tracking” or co-speciation [17, 18]. Comparative sequence analysis of multiple isolates of both barley and wheat powdery mildew pathogens, B. graminis f.sp. hordei (Bgh) and B. graminis f.sp. tritici (Bgt), revealed that at least their genomes are characterized by an ancient haplotype mosaic composed of isolate-specific DNA blocks, suggesting exceptionally rare outbreeding and dominant clonal reproduction of the haploid fungus in nature [12, 19].
Powdery mildew fungi have some of the largest genomes among plant-pathogenic Ascomycetes, strongly enriched with an unusually high content of transposable elements (TEs) [11, 12]. Extensive repetitive regions made up of TEs have hindered high quality short-read-based genome assemblies, resulting in severely fragmented datasets [6, 11, 12, 19]. The fragmentation of the available genomic assemblies has so far hampered our ability to address relevant biological questions, as for example the existence of long lineage-specific virulence regions, the impact of TEs on genome organization and evolution, as well as the conservation of gene order between diverged isolates.
In this study, we present a near-chromosome level assembly of the Bgh reference isolate (DH14), which recovers approximately 30 Mb of previously unassembled sequence, supplemented with a new, manually curated annotation. Genome-wide comparative analysis of the European DH14 isolate with the Japanese isolate RACE1, which is the most divergent Bgh isolate sequenced so far , revealed clear evidence for large-scale conservation of gene order between isolates. Subsequent comparisons with genomes of closely related B. graminis formae speciales indicated extensive copy number variation (CNV) of genes encoding secretion signal-containing proteins (SPs), which mirrors the phylogenetic relationships of these host-specialized forms. Finally, we found evidence for recent proliferation of TEs in the Bgh genome and possibly other formae speciales of B. graminis, but not in powdery mildews colonizing dicotyledonous host plants. Collectively, these genomic features reveal unprecedented insights into B. graminis life history and co-evolutionary patterns of the fungal pathogen with grass hosts.
Large-scale Bgh genome organization
To facilitate a deep exploration of the Bgh genome, we applied third generation long-read DNA sequencing to generate high-quality genome assemblies of a European and a Japanese isolate, designated DH14 and RACE1. Whilst a short-read-based genome is available for DH14 , enabling direct comparison with the newly established long read-based assembly, isolate RACE1 was chosen because of its exceptionally high coding sequence divergence compared to a collection of 15 other Bgh isolates from different geographic origins, including DH14 . Although the PacBio platform-based sequence depth for isolate DH14 was relatively low (~ 25×; Table 1), the Canu  assembly resulted in 963 contigs (i.e. 14,093 fewer contigs than the published reference genome), a significant increase of the N50 statistic (now 4.6 Mb), and an almost complete recovery of previously unassembled genomic sequences (Table 1). Using existing data from sequenced plasmid and fosmid clones , the assembly was further reduced to 318 scaffolds, comprising ~ 124.5 Mb in total. The final assembly was polished to remove erroneous base calls and insertions/deletions (indels) using short Illumina reads (~ 50× coverage). For isolate RACE1 the depth of the long read sequencing was higher (~ 50×) and thus these PacBio reads were used also for polishing. The resulting unscaffolded RACE1 assembly consists of 99 contigs (including the circular mitochondrial genome) and a total size of ~ 116.5 Mb (N50 3.9 Mb; Table 1). Overall, both assemblies show higher gene space coverage (BUSCO analysis) compared to the existing Bgh reference genome  although the difference is comparatively small (Additional file 1: Table S1). We did not find any evidence for the presence of previously reported Bgh-specific plasmid-like linear extrachromosomal DNA  in the two isolates.
To further assess assembly quality and to facilitate future genome-anchored genetic studies, we compared the assemblies with a previously generated genetic map for Bgh . We located genomic positions for 80 mapped single-copy expressed sequence tag (EST) markers and compared their physical linkage with the corresponding genetic map. This revealed in most cases (67 out of 80 ESTs) a collinear marker order on physical and genetic maps (Additional file 2: Figure S1). In all but two cases in which discrepancies were found between physical and genetic maps, we observed collinearity of EST markers between the independently assembled genomes of DH14 and RACE1. Even large genetic linkage groups were mostly covered by only one or two genome contigs (e.g. linkage groups 2 to 7; Additional file 2: Figure S1), suggesting that our physical maps partly represent Bgh chromosomes or chromosome arms. In support of this, we identified 19 (DH14) and 20 (RACE1) cases of canonical telomeric repeat sequences (5′-TTAGGG-3′ hexamer; 34 to 61 tandem copies) at the beginning/end of contigs, in some instances together with distally-located gene-scarce regions likely resembling centromeres (Additional file 3: Figure S2, Additional file 1: Table S2). The gene-scarce regions are in all cases associated with specific long interspersed nuclear elements (LINEs) of the Tad1 family (Additional file 3: Figure S2).
The circular mitochondrial genomes of both isolates were closed, yielding total sizes of 104 kb (DH14) and 139 kb (RACE1) (Additional file 4: Figure S3A), which is in agreement with older experimental estimates . Nucleotide sequence alignment indicated > 96% identity of the mitochondrial DNA (mtDNA) of the two genomes. It further revealed that the RACE1 mitochondrial genome contains a ~ 32 kb duplication, while the DH14 mtDNA encompasses an ~ 1 kb isolate-specific sequence stretch that includes one predicted open reading frame (Additional file 4: Figure S3B). The structural and nucleotide differences might be linked to the isogamous and hermaphroditic manner of mitochondrial inheritance in B. graminis , meaning that the mtDNA can originate from two parents derived from distant Bgh populations. Nonetheless, the Bgh mitochondrial genome does not present major differences in gene repertoires compared to known mitochondrial genomes of other Leotiomycetes , except for Atp9, which encodes the subunit 9/c of the mitochondrial ATP synthase complex and has been transferred to the nuclear Bgh genome. Consistent with this, Bgh Atp9 carries an N-terminal mitochondrial transfer signal sequence. This gene translocation has been observed in other fungal species and might be related to a physiological adaptation, enabling transcriptional modulation of its expression in cell- and tissue-specific contexts [26, 27].
Identification of isolate-specific genes, gene duplications and gene expression
Existing Bgh gene models for the isolate DH14 were transferred to the new assembly and were supplemented by new predictions generated by MAKER , which were guided by protein and/or transcript evidence (whole-transcriptome shotgun sequencing; RNA-seq; see Materials and Methods). For RACE1, for which a prior genome annotation was unavailable, we generated de novo gene models using MAKER, guided by protein and transcript evidence from both Bgh isolates. We manually curated all gene models, removed poorly supported predictions, presumptive pseudogenes (mostly related to Sgk2 kinase-like genes; ) and annotations that overlapped with TEs. During the manual curation we noted several instances of (tandem) duplicated genes, which are highly sequence-related at the nucleotide level, and thus had been collapsed into single gene models in the previous DH14 genome assembly . This complicated the annotation and therefore new gene identification numbers (IDs) were generated also for DH14 (Additional file 1: Table S3).
The new annotation resulted in 7118 gene models for DH14, of which 805 genes encode predicted SPs. A similar number of 7239 gene models were found for RACE1 upon manual curation, including 770 that encode predicted SPs. A subgroup of SPs, called CSEPs, are secreted candidate virulence proteins defined by specific criteria . For a more comprehensive coverage of the deduced fungal secretome, we generally included all SPs in our analyses. This also allowed us to incorporate newly detected effector candidates resulting from the re-annotation of the Bgh genome.
To compare the gene repertoires encoded by the DH14 and RACE1 isolates, we first used OrthoFinder to infer orthologous gene groups (orthogroups). This analysis identified 6039 single-copy groups containing gene pairs with unambiguous one-to-one relationship between the isolates (Fig. 1a). By manually incorporating additional position and synteny information from a whole-genome alignment (see below) for the inference of orthologous gene pairs, we could further resolve some ambiguities and identify additional relationships for unassigned genes with more dissimilar sequences, significantly increasing the number of one-to-one gene pairs to 6844 (Fig. 1b, Additional file 1: Table S4). A comparison of DH14 and RACE1 orthogroups showed that most groups (6200 out of 6319) contain the same number of members in both isolates, but there are several groups with an isolate-specific expansion, indicating the presence of additional paralogs in one of the isolates (Fig. 1c, Additional file 1: Table S4). Such isolate-specific expansions occur almost 10-fold more frequently for SP-containing groups than for groups without SPs (9.4 and 1.2%, respectively; χ2-test, p < 2e− 16). An example for the occurrence of such an isolate-specific gene duplication is the AVR a1 avirulence effector  for which two identical copies exist in DH14, while only one copy was found in RACE1 (Additional file 5: Figure S4A). By contrast, the AVR a13 avirulence effector locus is highly similar in both isolates, with a single copy of AVR a13 flanked by the other two members of the previously identified AVR a13 CSEP family [9, 13] (Additional file 5: Figure S4B).
We also searched for isolate-specific genes without any related sequence in the other respective isolate. For this purpose, we included the previously published RNA-seq data for RACE1  and a corresponding newly generated dataset for DH14 as additional evidence to extract a high-confidence set of isolate-specific genes. This analysis identified in total 31 isolate-specific genes in DH14, for 13 of which we detected credible gene expression (FPKM (fragments per kilobase [sequence length] and million [sequenced fragments]) ≥ 5) during pathogenesis (Additional file 1: Table S5). A similar number of 27 isolate-specific genes was found in RACE1, of which 19 were also expressed (FPKM≥5) during pathogenesis (Additional file 1: Table S5). Among these expressed isolate-specific genes, we found eight SPs in DH14, but only three in RACE1. As the two isolates are of opposite mating types, also the corresponding MAT idiomorphs were among the isolate-specific genes, with DH14 carrying MAT1–2-1 and RACE1 carrying both MAT-1-1-1 and MAT-1-1-3 (Additional file 1: Table S5, Additional file 6: Figure S5).
Apart from a validation of the presence of isolate-specific genes, the RNA-seq data enabled us to examine also potential isolate-specific gene expression during infection. We searched for orthologous gene pairs for which we could detect robust transcript levels (FPKM≥10) in one of the two isolates while in the other the corresponding gene was not expressed (FPKM< 1 or raw count≤2), and for which isolate-specific expression could be further validated by visual inspection in the Integrative Genomics Viewer (IGV; ). A total of 15 genes showed differential expression based on these criteria (Additional file 1: Table S6). Of these genes, 12 were specifically expressed in RACE1 (of which seven encode CSEPs), while three were expressed specifically in DH14 (Additional file 1: Table S6), indicating manifest differences in expressed gene repertoires between Bgh strains.
Genome synteny, structural and sequence variation between isolates
For a detailed genomic comparison, we conducted a whole-genome alignment of DH14 and RACE1 assemblies using MUMmer . Although RACE1 was chosen for genome sequencing based on its high sequence divergence to DH14 within coding regions , the genomes of the two isolates overall are still remarkably similar, with 92 and 98% of the assemblies of DH14 and RACE1 aligning to the corresponding other isolate at an average nucleotide sequence identity of ~ 99%. Moreover, the aligned sequence stretches form large syntenic blocks of up to 9 Mb, implying that gene order within the assembled contigs is also largely conserved between the isolates (Fig. 2a). A closer inspection of the syntenic blocks revealed that the large-scale synteny between DH14 and RACE1 can be interrupted locally by intermittent stretches of non-syntenic alignments (e.g. to a different contig in the other isolate) or by sequence areas without a close match in the other genome (Fig. 2b). These interspersed alignment gaps typically are rather small (< 1 kb on average) and concern primarily regions of repetitive sequence, while only rarely affecting protein-coding genes (only 1% of alignment gaps affect genes). As both genomes are not resolved entirely to whole-chromosome level, we cannot estimate the full extent of large-scale chromosomal reshuffling. Nevertheless, the occurrence of within-contig alignment breaks provides evidence for at least two large-scale genomic rearrangements that involve genome stretches larger than 1 Mb (Fig. 2a, Additional file 7: Figure S6). Additionally, we found 128 cases of genomic rearrangements within contigs, where sequence stretches of at least 10 kb are inverted relative to the other isolate. These inversions occur dispersed throughout the genome and the average size of inverted regions is around 20 kb with only seven regions larger than 50 kb. Roughly half of these local inversions (69 out of 128) affect gene-containing regions, but only for 22 of the corresponding regions we could verify by manual screening that they coincide with an inverted gene order relative to the flanking genes (Fig. 2c, Additional file 1: Table S4). In three of these cases, a further re-shuffling of genes was observed within the inverted region. Collectively, while large parts of the genome structure and gene order seem to be well conserved, we detect a number of mostly smaller synteny breaks that are dispersed throughout the genome and contribute to the structural variation between the two isolates.
To examine the sequence variation between RACE1 and DH14, we used the single nucleotide polymorphisms (SNPs) identified in the MUMmer  dnadiff analysis to calculate SNP frequency in 10 kb sliding windows. In addition, we obtained SNPs for isolates A6 and K1  from a short-read-based alignment (see Methods) and calculated the corresponding SNP frequencies to re-examine the sequence variation of these isolates to the improved DH14 reference genome. On average, the overall SNP frequency is three times higher in RACE1 (4.7 SNPs/kb) than in A6 (1.4 SNPs/kb) and K1 (1.3 SNPs/kb). Moreover, a comparison of SNP frequency distributions between the three isolates shows that in RACE1 SNP frequencies below one SNP per kb are seen only rarely, whereas in A6 and K1 they are common (Additional file 8: Figure S7A). Accordingly, a two-component mixture model fitted to the observed SNP frequencies recovered the previously described  distinction between low and high SNP densities (mean ± standard deviation) for A6 (low: 0.1 ± 0.1; high: 1.9 ± 1.5) and K1 (low: 0.1 ± 0.1; high: 2.0 ± 1.7). By contrast, for RACE1 no such distinction could be observed and the SNP frequency was high for both model components (low: 3.8 ± 2.4; high: 10.6 ± 6.1; Additional file 8: Figure S7B).
SP paralogs typically reside in close proximity
Although local clustering – in part even as tandem duplicates - of genes encoding effector candidates in the Bgh genome has been suggested and described , its scale at a genome-wide level remained unclear. This is mainly due to the severe fragmentation of the previously available genomic assemblies and the collapse of highly similar gene copies in the short-read-based assemblies [11, 19]. We therefore explored systematically whether SPs in general co-occur in close distance. Here we defined SP clusters based on two criteria: (1) each cluster contains at least three SPs and, and (2), two SPs are separated by a maximum of ten genes coding for non-secreted proteins. By these criteria, 72% of the SP-coding genes (583 out of 805) can be placed in three large clusters with more than 30 SPs and 74 smaller clusters with less than 20 SPs (Additional file 1: Table S7). Consistent with an earlier study , many of these clusters harbor sequence-related genes which belong to the same orthogroup (Additional file 1: Table S7), suggesting that they might originate from recent local duplications with subsequent sequence diversification, thus likely representing paralogs. Despite this occurrence of SP clusters, we did not observe local enrichment of SPs on particular genomic scaffolds (Additional file 9: Figure S8A). Rather we found that the SP count follows the scaffold size (Additional file 9: Figure S8B), which is in line with the results of a χ2-test that did not detect a significant deviation between the SP frequency per scaffold and the underlying genome fraction per scaffold (p = 0.21).
Copy number variation of SPs within and between formae speciales correlates with phylogeny and host specialization
To investigate the extent of within-genome gene duplications we used MCScanX  on the DH14 and RACE1 isolate datasets. As expected for a haploid genome, the majority of the genes exist in single copies, but ~ 10% have one or more paralogs (Additional file 1: Table S8). Approximately one third of these duplications occur in tandem (36%), while the remaining ones are either proximal (in-between the next five genes) or dispersed throughout the genome (30 and 33%, respectively). When compared to the genomes of the phylogenetically closely related phytopathogenic fungi Botrytis cinerea and Sclerotinia sclerotiorum, the Bgh genome shows a higher percentage of duplications (11% versus 0.3 and 5.4%, respectively). A closer look at the S. sclerotiorum dataset revealed that the seemingly elevated number of dispersed and proximal duplications in this species is mainly comprised of retrotransposases that are retained in the corresponding annotation (Additional file 1: Table S9). This finding indicates that the comparatively high number of paralogous gene pairs (812 out of 7118) in the Bgh genome is a unique characteristic among the so-far-sequenced Leotiomycetes.
We investigated whether these duplications can be associated with certain types of genes or functional domains and found that SP genes are significantly more subject to duplication than genes encoding non-SPs (χ2 test, p < 0.001). Most duplications of SPs seem to occur in tandem (Additional file 1: Table S10). Functional domain associations are poor for the group of SP genes because effector proteins often have few or no functional descriptions (applies to ~ 79% of the 805 predicted SPs in DH14 in PFAM-based searches; Additional file 1: Table S11). However, there are two clusters with tandemly duplicated genes that are rich in genes encoding ribonuclease-like domains (SUPERFAMILY SSF53933, clusters 21 and 1), and two clusters with Egh16 virulence factor homologs (PFAM PF11327, clusters 56 and 14). Among the genes coding for non-SPs, a portion of the duplications (181 out of 546) are related to genes with kinase-like domains (SSF56112, PS50011), which have been described previously as an over-proliferating family in the Bgh genome .
Based on the above results we sought to determine whether gene copy numbers vary between strains belonging to different formae speciales of B. graminis. Using published datasets [12, 16, 18, 19], we estimated the copy number of each SP based on the observed coverage of short-read-based sequence alignments against the DH14 assembly (Fig. 3a). To assess the accuracy of this analysis, a sample of genes with tubulin or actin functional domains and some additional non-SP-coding genes with conserved domains was used. As expected, this control dataset showed minimal variation and revealed conserved single-copy presence in all 52 genomes examined (representing 9 formae speciales; Additional file 10: Figure S9), indicating that the analysis based on coverage depth is robust. Nonetheless, false approximations cannot be fully excluded by this approach.
For the majority of SPs (458 of 805; 57%) we detected simple presence/absence variation between the different formae speciales and their respective isolates (Fig. 3a). For a smaller fraction of SPs (201 of 805; 25%) the number of observed copies varies between 0 (absence) and more than 2 copies per genome. Interestingly, while variation in copy numbers between the examined genomes can be observed (Fig. 3a), for many SPs (72–87%, depending on the forma specialis) the number of gene copies is conserved among different isolates of the same forma specialis (e.g. BLGH_01048 has 2 copies in all f.sp. secalis and f.sp. dicocci genomes). In addition, high-copy SPs have low sequence similarity with each other (Fig. 3a). To investigate whether CNV correlates with the phylogeny of the formae speciales, we generated a tanglegram using a dendrogram derived from the hierarchical clustering of the CNV data and a cladogram derived from a UPGMA tree based on ~ 1.07 million single nucleotide polymorphism (SNP) positions between the isolates (Fig. 3a). The CNV-based dendrogram accurately groups the isolates based on their host specificity, indicating that isolates belonging to the same formae speciales have distinctive CNV profiles.
The Blumeria core effectorome
To define the core effectorome of the species B. graminis, we de novo-assembled and annotated the genomes of single isolates of the 9 formae speciales and inferred orthology relationships for the predicted proteomes. Our amino acid sequence-based orthology clustering of the predicted SPs (Additional file 11: Figure S10A) suggests that although part (see below) of the secretome is highly conserved in all formae speciales, another subgroup is divergent. Also, due to the divergence at the DNA sequence level the presence of certain SPs in the genomes of the more distantly related formae speciales avenae, lolii and poae was not detectable in the short-read-based CNV analysis above (Fig. 3a), while the orthology analysis identified related sequences at the amino acid level (Additional file 1: Table S11). Yet, the formae speciales avenae, lolii and poae still share smaller intersections with the Bgh secretome compared to the rest (Additional file 10: Figure S10A).
Out of the 805 Bgh SPs present in isolate DH14, 442 have at least one ortholog in all genomes assayed. A considerable fraction of these widely conserved SPs (252 out of 442; 57%) has PFAM domains and/or homologs outside the Blumeria genus. As indicated by their functional annotation (e.g. peptidases/proteases, hydrolases), these SPs are rather part of a common SP repertoire of fungal plant pathogens and are not specific innovations of the grass powdery mildews. On the other hand, 190 SPs fulfil the typical CSEP criteria (no homology outside the Erysiphales, no PFAM domain; ) and can be considered as the core effectorome of the grass powdery mildews. These core CSEPs belong to different phylogenetic families (Additional file 10: Figure S10B), possibly targeting a core set of conserved host functions to maintain virulence on grasses.
The Bgh genome exhibits no obvious compartmentalization
Various types of TEs that are dispersed more or less evenly throughout the genomes (Fig. 4a, Additional file 1: Table S11) dominate the intergenic space of the DH14 and RACE1 genomes. Accordingly, many TEs can be found in close vicinity to genes, regardless if they are coding for SPs or not (Fig. 4a). This pattern contrasts with other sequenced fungal and oomycete plant pathogens where transposon-rich areas are essentially limited to lineage-specific regions/chromosomes or are largely confined to isochores [33, 34]. Several copies of these elements seem to be expressed, in particular certain types of Copia elements (Additional file 1: Table S12), and in many cases, overlap with the 5′ or 3’ UTRs of nearby genes (Fig. 4a).
A complementary analysis of the local gene density, measured as flanking distances between neighboring genes, shows that in general the flanking distances in the Bgh genome are rather high, with an average distance of ~ 14 kb (Fig. 4b). Accordingly, the surrounding genomic context of most genes in the Bgh genome is gene-sparse and repeat-rich and large flanking distances are not specific to SP genes (Fig. 4b). In line with this pattern, also the flanking distances of the two known Bgh AVR effector genes, AVR a1 and AVR a13 , are not exceptionally large compared to the overall genome (Fig. 4b). We further investigated whether genes coding for CSEPs or other SPs, which do not fulfil the typical effector criteria, present a difference in their 5′ or 3′ intergenic distances compared to ascomycete core ortholog genes (COGs). Regarding the 5′ intergenic distances, we detected no marked variation between the groups (ANOVA, p = 0.382), while the 3′ intergenic distances on average were slightly larger for the COGs than for both the CSEPs and other SPs and (ANOVA, p = 0.004; Tukey post hoc tests, p < 0.05; Additional file 3: Figure S2B). The results of this analysis highlight that in Bgh CSEPs or other SPs are not located in peculiar gene-scarce regions compared to the conserved COGs. In addition, low gene density also could not be associated with high dN/dS rates (Additional file 3: Figure S2C), indicating that fast evolving genes in Bgh such as the CSEPs can occupy both gene-rich and gene-scarce areas. Thus, the Bgh genome does not appear to be split into distinct compartments, but is rather characterized by a low gene density and high TE density throughout the entire genome.
A recent lineage-specific TE burst shaped the Bgh genome
Since TEs occupy the majority of the Bgh genome and are in many cases closely entangled with presumed virulence genes (SPs), we examined whether these repetitive sequences slowly accumulated over time or, alternatively, were subject to sudden expansions in the life history of powdery mildews, which might be linked to the observed proliferation and clustering of some highly sequence-related SPs. We used RepeatMasker (www.repeatmasker.org) to detect TEs with previously curated annotations found in Repbase (http://www.girinst.org/about/repbase.html), and subsequently generated repeat landscapes based on the divergence from the corresponding consensus TE sequences.
Surprisingly, most of the repetitive elements in Bgh show very low nucleotide sequence divergence (< 10%) compared to the TEs in 13 closely related Leotiomycete genomes (typically 30–40% nucleotide sequence divergence; Fig. 5a, b), suggesting a recent lineage-specific expansion of TEs within Bgh (Fig. 5b, c). In addition, there are 1866 occurrences of long terminal repeats (LTRs) with less than 0.1% divergence associated with either Gypsy or Copia elements (~ 3% of the LTRs than can be identified), indicating that the Bgh genome carries very recent transposition events. Finally, the observed TE expansion in Bgh can be equally attributed to both LINE and LTR retrotransposons (Fig. 5c). As outlined above, for part of these TEs, in particular Copia elements, evidence of expression can be found in the RNA-seq datasets (Additional file 1: Table S12).
Genome assemblies of B. graminis isolates belonging to other formae speciales, which are exclusively based on short reads, were found to underestimate both the magnitude of TE expansion and the presumed divergence time. This is due to the fact that the majority of the highly similar repetitive sequences collapse into few contigs, as revealed by the comparison of Bgh assemblies that are either based on long (PacBio) or short reads (Illumina; Additional file 12: Figure S11A). Therefore, for the other formae speciales of B. graminis it can only be assumed that they also experienced a recent TE expansion, while it remains unclear whether this event is older or more recent than the one in Bgh.
Remarkably, when applying the same pipeline on the sequenced genomes of the dicot-infecting powdery mildews Erysiphe necator, E. pisi and Golovinomyces orontii, the divergence from the consensus of the respective TE sequences is much higher (25–35% compared to < 10% in Bgh), suggesting that the expansion of the repetitive elements in these species is more ancient than in Bgh (Additional file 12: Figure S11B). This calculation is unlikely to be an underestimation due to the short-read-based genome assemblies of these species as long-(PacBio) or short-read-based assemblies revealed similar divergence rates for G. orontii. Because evolutionary rates within the Erysiphaceae family appear to be comparable [35, 36] and essentially all TEs in dicot-infecting powdery mildews are sequence-diverged (> 10%; Additional file 12: Figure S11B), this observation suggests independent “transposon bursts” for each powdery mildew lineage that occurred at different times.
An improved assembly provides insights into large-scale organization of the Bgh genome
The genome of the obligate biotrophic pathogen Bgh is characterized by a loss of genes encoding enzymes of primary and secondary metabolism as well as an expansion of overall genome size due to a massive proliferation of TEs . This high repeat content, with TEs representing more than two thirds of the genome, makes it essentially impossible to generate chromosome-level DNA assemblies from short sequencing reads that do not allow to resolve these highly similar sequences. Accordingly, the first short-read-based assembly for Bgh isolate DH14 was highly fragmented, with more than 15,000 contigs (and close to 7000 scaffolds), and about one third of the estimated genome size was not covered , possibly due to collapsed sequences.
We here used a single-molecule sequencing technique to generate long DNA sequence reads, which enabled us to establish high quality genome assemblies for the two Bgh isolates, DH14 and RACE1. For DH14, this long-read-based assembly showed a > 10-fold improved contiguity and recovered a substantial amount of previously unassembled genomic sequence (50% increase in genome size) compared to the first genome draft. In both DH14 and RACE1 assemblies, the largest contigs are more than 9 Mb in size, likely to represent complete chromosome arms, and a similar number of observed telomeric repeat regions in both assemblies (19 and 20) suggests the Bgh genome is likely partitioned into 10 chromosomes.
The high assembly quality is also supported by both an improved gene space coverage (now > 98% BUSCO coverage for the newly annotated DH14 reference genome; Additional file 1: Table S2) and good agreement with a previously published genetic map of Bgh . The yet missing BUSCOs could be due to either real gene loss events or failure to detect the corresponding conserved ortholog by the software, suggesting that the core gene space is now essentially completely covered in the Bgh reference genome. The few observed discrepancies between physical contigs and the genetic map might be attributed to the fact that the linkage map was constructed from a cross between two isolates (C15 and JEH31) that are different from the ones used in this work. Therefore, while we cannot exclude that the few discrepancies are at least partly due to remaining inaccuracies in either our assemblies or the genetic map, these also could be evidence for additional isolate-specific genomic rearrangements.
Effector repertoires differ slightly between the two Bgh isolates
Approximately 74% of both assemblies are made up of repetitive elements that are uniformly dispersed across the genome, which is an even higher repeat fraction than predicted before for Bgh (64%; ). The previous underestimation of the TE content could be due to the collapse of highly repetitive short-read-based sequences during genome assembly. While a comparable fraction of TEs was described for the oomycete pathogen P. infestans , other sequenced fungal genomes contain markedly lower fractions (Fig. 5b; ).
In addition to a drastically improved assembly of repetitive sequences, we also noticed the existence of loci with similar or identical copies of a number of genes, which had previously been collapsed into single gene models (Additional file 1: Table S3). Thus, genome re-annotation based on the new assemblies also provided an improved representation of Bgh gene repertoires, increasing the number of gene models from 6470  to 7118 in the annotation of the reference isolate DH14. A subsequent comparison of protein-coding genes between DH14 and RACE1 revealed largely conserved gene numbers between the two isolates, which is in agreement with previous observations based on short-read-based assemblies of three Bgh isolates . However, due to the improved resolution, here we were able to identify several cases of isolate-specific gene family expansions and gene duplications, especially affecting SPs. Moreover, we identified several SP genes that were present exclusively in one of the genomes and lacked any similar sequence in the other isolate. The observed differences suggest that diversity of SP repertoires in Bgh is maintained mostly through gene duplications with subsequent sequence diversification and gene deletions. Thus, our observations for Bgh reflect the general evolutionary pressure on pathogen populations to diversify effector repertoires, which could then serve as reservoirs for rapid adaptation in response to population-level alterations in host R genes. Accordingly, the diversity of Bgh effectors is important in balancing the trade-off between ensuring virulence function and, at the same time, trying to escape detection by the host plant .
Interestingly, the gene with the strongest isolate-specific expression in RACE1 encodes thioredoxin A, which is important for protection from oxidative stress and contributes to virulence of human pathogenic bacteria and fungi [40, 41]. However, as the RNA-seq samples for RACE1 and DH14 were generated in different experimental batches, we cannot fully rule out the possibility that the expression differences we observed could be partially influenced by batch effects.
TEs and SPs are evenly dispersed throughout the genome
Many filamentous pathogens exhibit a distinct genome architecture, denoted as “two-speed genome”, with well-defined blocks of low gene and high TE density, interspersed between the generally more prevalent genomic areas of high gene and low repeat content [42,43,44]. These TE-rich blocks, which often harbor genes encoding secreted effector proteins, typically exhibit high lineage-specific diversity and are prone to be involved in genomic rearrangements [42, 43, 45]. In this way, these regions are thought to provide a pool of genetic variation that is needed by phytopathogens to quickly adapt to changing requirements in the evolutionary arms race with their hosts .
In Bgh, however, the situation is clearly different, as the numerous TEs are not restricted to specific areas, but rather evenly dispersed throughout the genome (Fig. 2a, Additional file 9: Figure S8A). In addition, neither are the flanking regions of SPs particularly enriched in TEs, nor are they markedly larger compared to non-SPs (Fig. 4a, b). Moreover, SPs, whether they are categorized as putative effectors (CSEPs) or not, are not associated with unusually gene-sparse (Additional file 3: Figure S2B) or peculiar genomic regions (Additional file 9: Figure S8A), but their number is positively correlated with scaffold size (Additional file 9: Figure S8B). Additionally, the dN/dS ratio of the CSEPs is not associated to local gene density (Additional file 3: Figure S2C).
We also did not detect any large lineage-specific regions as reported for Verticillium dahliae . Instead, smaller lineage-specific (< 1 kb on average; up to 51 kb) or locally inverted (< 20 kb on average; up to 90 kb) sequence stretches can be found dispersed rather evenly distributed throughout the genomes of the two Bgh isolates. Thus, the organization of the Bgh genome does not match the “two-speed genome” model , in which genetic variation is concentrated in specific genomic areas. Instead, Bgh appears to have a “one-speed/high-speed genome” where genetic and structural variation is not tied in specific compartments but rather sustained throughout the whole genome. Such a genome architecture might contribute to maintaining genetic diversity of mainly asexually reproducing Bgh. However, in this scenario genomes would be expected to rapidly lose the overall synteny due to TE activity and cumulative effects of local genome rearrangements. Thus, it is conceivable that occasional sexual reproduction ensures the maintenance of overall synteny of Bgh genomes.
Our present work supports the assumption of a predominantly asexual reproduction mode in Bgh, as we were able to recover the previously described mosaic genome structure in the European Bgh isolates (A6, K1 and DH14), with isolate-specific alternating regions of low and high sequence diversity  (Additional file 8: Figure S7). For the highly divergent Japanese isolate RACE1, on the other hand, no monomorphic regions were detectable relative to DH14 (Additional file 8: Figure S7), which is most likely due to the prolonged geographic separation of the two isolates during which sequence variation could accumulate at a whole-genome scale.
Grass powdery mildews have a fast-paced secretome adapted to their respective hosts
Effector proteins play a crucial role in interactions between plant pathogens and their respective hosts , and consequently both small (sequence divergence) and big (loss of effector clusters) changes can drive the preference of the pathogen to a new host . To date, several genome reports have established that phylogenetically related pathogens share a core effectorome, whereas each member of a taxonomic lineage contributes its own unique effectors to the pan-effectorome [48,49,50]. The large number of candidate effectors in the core effectorome of the Blumeria genus identified here, including at least 190 CSEPs belonging to 74 gene families, suggests these are indispensable for the maintenance of fungal virulence on different monocotyledonous hosts in each forma specialis of the species B. graminis. Whether the corresponding effector families mainly target different host components belonging to few or a large number of cellular pathways for the establishment of a biotrophic relationship with their grass hosts remains to be tested.
One interesting aspect of the grass powdery mildew effectorome is the CNV that some of its members experience (Fig. 3a, b). As in other plant pathogens, this variation is dominated by presence/absence polymorphisms , indicating strong selection for some SPs by certain host genotypes. In addition, we noted increased numbers of SP copies in particular isolates and formae speciales, suggesting that transcript dosage might also play a role in host adaptation of powdery mildews. In other plant pathogens, increased copy number of virulence genes can alter the infection phenotype, as for example reported in the case of ToxB in Pyrenophora tritici-repentis [51, 52].
For powdery mildews this evolutionary pattern might be particularly advantageous because the loss of the repeat-induced point mutation mechanism (RIP; ) allows additional gene copies to remain intact and functional , providing a presumed fitness advantage. This can be for example observed in Erysiphe necator, where an increased copy number of EnCYP51 enhances fungicide resistance . Similarly, careful re-examination of existing data using the information from the new Bgh reference assembly indicates that for some isolates duplications of CSEPs could offer the means to escape detection by their respective host via naturally accumulating mutations in one of the copies. An example of this might be AVR a1 , where one of the two copies present in isolate CC107 has accumulated mutations allowing evasion of detection in barley cultivars carrying the matching Mla1 R gene . A recent report  suggests extensive forma specialis-specific expansions of certain CSEP families, supporting the conclusions of our CNV and SP orthology analysis (Fig. 3a, Additional file 11: Figure S10A).
TEs expanded suddenly and massively in the Erysiphaceae
The Bgh genome is frequently referred to as a typical example of repeat-based expansion of an eukaryotic genome . Even early studies predating high-throughput genome sequencing revealed that the effect of TEs in this pathogen’s genome is significant. This conclusion was based on the frequency these sequences are associated with coding regions [56,57,58]. Nevertheless, the question of whether the activity of TEs and their dominance in the genome has been a beneficial or a neutral feature is still open.
TEs in the genome of Bgh are evenly distributed, in part transcriptionally active and flank virulence genes as much as genes involved in all types of basic biological processes (Fig. 2a, Additional file 3: Figure S2, Additional file 9: Figure S8A). As in many other cases, it can be hypothesized that TEs can act as templates for rearrangements, deletions and duplications of genomic sequences [42, 49]. Furthermore, TE insertions next to or within virulence genes can change the pathogen’s host range [59, 60].
We show for the first time that TEs in the grass-infecting (Blumeria) and dicot-infecting (Erysiphe) powdery mildews experienced sudden and, in evolutionary terms, synchronous expansions. Taking into consideration molecular clock studies [18, 36], it is tempting to hypothesize that TE bursts in the genomes of Erysiphaceae occurred independently of each other and might have preceded or followed adaptation to new hosts. Similar observations placing TE bursts around speciation times have been reported in the plant pathogen Leptosphaeria maculans [33, 61] and other eukaryotic organisms . Theoretical models suggest that sudden TE expansions, when seen as a source of mutations, can push asexual organisms to a fitness optimum in adverse conditions [63, 64]. Given that at least powdery mildews of the genus Blumeria reproduce mainly clonally (asexual) as haploid organisms [12, 19] and their formae speciales exhibit narrow host specificity, our findings call for future studies to clarify the relationship between TE expansion and changes in the pathogen’s host range.
We provide a greatly improved reference (isolate DH14) resource for the barley powdery mildew pathogen, and a near-continuous assembly of the highly divergent isolate RACE1. Gene order between these two isolates is retained at large scale, but locally disrupted. Using the new reference and supplementary transcriptomic and genomic data, we reassessed the secretome of grass powdery mildews and defined a core group of 190 SPs, which are likely to be indispensable for virulence. Inter-formae speciales comparisons further revealed that these virulence-related genes exhibit extensive CNV and sequence divergence, which reflects the phylogeny of these powdery mildews. SP genes are often locally clustered, but these clusters are evenly dispersed throughout the genome. TEs, which like the SP clusters are uniformly distributed in the Bgh genome and in part actively transcribed, experienced a recent lineage-specific expansion.
Taken together the results presented here indicate that Bgh, and more broadly the species Blumeria graminis, has a highly dynamic genome. While for other filamentous pathogens the existence of a “two-speed” genome has been suggested, the characteristics of the Bgh genome (even genome-wide distribution of TEs and SPs) indicate a “one/high-speed” genome for this pathogen and possibly its close relatives. It remains to be shown whether and how these features were enabled by the loss of genome defense modules (e.g. RIP), and if they contributed as springboard for the conquest of new host species (host jumps and host range expansions).
For DH14, genomic DNA was extracted as described in , while for RACE1 the protocol described in  was used. Subsequently, SMRTbell™ genomic libraries were generated and sequenced at the Earlham Institute (formally known as The Genome Analysis Centre, Norwich, United Kingdom) and at the Max Planck Genome Centre in Cologne (Germany) for DH14 and RACE1, respectively. The Pacific Biosciences (PacBio) RSII sequencing platform with either P5C3 (DH14) or P6C4 (RACE1) chemistry was deployed (Pacific Biosciences, Menlo Park, CA; ). A total of 21 SMRT cells achieved ~ 50× coverage for RACE1 (1,115,202 reads, 8357 bp average size), while for DH14 6 SMRT cells resulted in ~ 25× coverage (1,478,871 reads, 4540 bp average size). In addition, DH14 genomic DNA was sequenced at ~ 50× coverage with the Illumina MiSeq platform, providing 2 × 300 bp paired-end reads.
For both isolates the obtained PacBio reads were trimmed, corrected, and assembled using the Canu assembler (version 1.4; ) with default settings. The RACE1 assembly was further polished using Quiver (version 0.9.0; ) with default parameter settings. In the case of DH14 the resulting contigs were scaffolded with BESST (version 2.2.5; ) using previously published plasmid and fosmid libraries  and then polished using Illumina short reads and Pilon (version 1.18; ). To assess completeness of both assemblies we applied BUSCO (version 2.0.1; ) with default parameters searching against the Ascomycota database (ascomycota_odb9). To compare the assemblies with a previously published genetic map for Bgh , we obtained the nucleotide sequences of 80 single copy EST markers from this study and used BLASTN (BLAST+ version 2.3.0; ) to map these sequences against our genome assemblies (with e-value 1e− 6), thereby revealing their genomic location.
RNA sequencing and alignment
For RACE1, we used RNA-seq data generated in the context of a previous study , and for DH14 we generated corresponding samples from barley leaf epidermal peels at 16 and 48 h after Bgh conidiospore inoculation for RNA-seq as described before . The RNA-seq libraries were prepared by the Max Planck Genome Centre in Cologne (Germany) using the Illumina TruSeq stranded RNA sample preparation kit. The resulting libraries were subjected to paired-end sequencing (150 bp reads) using the Illumina HiSeq2500 Sequencing System.
To assess gene expression in DH14 and RACE1, the RNA-seq reads from both isolates were mapped to both genome assemblies under consideration of exon-intron structures using the splice aware aligner TopHat2  with adjusted settings (−-read-mismatches 10 --read-gap-length 10 --read-edit-dist 20 --read-realign-edit-dist 0 --mate-inner-dist 260 --mate-std-dev 260 --min-anchor 5 --splice-mismatches 2 --min-intron-length 30 --max-intron-length 10,000 --max-insertion-length 20 --max-deletion-length 20 --num-threads 10 --max-multihits 10 --coverage-search --library-type fr-firststrand --segment-mismatches 3 --min-segment-intron 30 --max-segment-intron 10,000 --min-coverage-intron 30 --max-coverage-intron 10,000 --b2-very-sensitive) to account for sequence variability between isolates. To assess the expression of individual genes, we obtained raw fragment counts per gene from the mapped RNA-seq reads for both isolates (summarizing both time-points) using the featureCounts function (−t CDS -s 2 -M -p) of the Subread package (version 1.5.0-p1; ) and subsequently normalized these raw counts to fragment counts per kilobase CDS per million mapped reads (FPKM) for better comparability.
Expression of TEs in the isolate DH14 was assessed by mapping pooled RNA-seq reads coming from the 16 and 48 hpi DH14 samples with STAR , using the RepeatMasker-derived gff file as annotation. Raw counts per TE annotation were obtained using the --quantMode GeneCounts option.
The prediction of DH14 and RACE1 gene models was performed using the MAKER pipeline (version 2.28; ), which integrates different ab initio gene prediction tools together with evidence from EST and protein alignments.
For DH14, initially the previous gene models (v3, https://www.ebi.ac.uk/ena/data/view/GCA_000151065.3) were transferred to the new assembly as described . Then an additional round of annotation followed, incorporating ESTs assembled from public Bgh datasets (Additional file 1: Table S13) using Trinity , protein datasets (Additional file 1: Table S13), as well as trained prediction models for AUGUSTUS , SNAP  and GeneMark-ES  as supporting evidence. All the annotations were subsequently manually curated using Web Apollo , removing unsupported gene models.
For RACE1, we performed a complete de novo annotation, as there were no previous gene models available. For this purpose, the MAKER pipeline was first run using AUGUSTUS  with species model Botrytis cinerea and GeneMark-ES  for ab initio gene prediction together with transcript and protein alignment evidence. The corresponding alignment evidence was created from BLAST and Exonerate  alignments of the DH14 protein sequences as well as RACE1 protein and transcript sequences. The RACE1 transcript and protein sequences for these alignments were obtained from the corresponding RNA-seq data via a transcriptome de novo assembly using Trinity  with default parameter settings for paired-end reads and subsequent open reading frame/peptide prediction using TransDecoder  with default settings. The resulting gene models from the first MAKER run were used as initial training set for another ab initio prediction tool, SNAP . Next, the annotation pipeline was re-run including all three ab initio prediction tools together with the transcript and protein alignment evidence, thus generating a second, improved training set for SNAP. After re-training SNAP on this set, the complete annotation pipeline was run a third time to yield the final RACE1 gene models. For both isolates, the obtained gene models were manually curated using Web Apollo , to correct for errors and remove poorly supported gene models. The mitochondrial genome of DH14 was annotated using RNAweasel and MFannot (http://megasun.bch.umontreal.ca/RNAweasel/).
Identification of orthologous genes and gene groups
Groups of orthologous genes (orthogroups) were inferred from DH14 and RACE1 using OrthoFinder (version 1.1.8; ) with the inflation value I set to 1.2. To further resolve ambiguities in the orthogroups and detect additional relationships between more dissimilar sequences, subsequently, a manual screening of gene positions and co-linearity in the two genomes was performed and the ortholog assignment was refined accordingly.
Isolate-specific genes were identified by combining the results of the OrthoFinder analysis with the alignment results for the RNA-seq data from both isolates. Explicitly, a gene was only considered to be specific for one isolate if, after OrthoFinder analysis and manual refinement, there was no orthologous gene detectable in the genome of the other isolate and additionally also no RNA-seq fragment (read pair) from the other isolate were detected to map against this gene (raw count ≤1). The fragment count per gene was calculated from the mapped RNA-seq read pairs (with mapping quality > 0) using featureCounts (version 1.5.0; ) with adjusted settings (−s 2 -p -M), based on the curated gene models. For identification of isolate-specific gene expression the raw fragment counts were further normalized to FPKM values, to adjust for potential differences in coding sequence length and RNA-seq read depth between isolates.
To calculate non-synonymous (dN) and synonymous (dS) substitution rates between DH14 and RACE1, we first aligned the protein sequences for each of the manually curated orthologous gene pairs with ClustalW (version 2.1; ). Subsequently, the protein alignments were converted to codon alignments using PAL2NAL (version 14; ) and dN and dS rates were estimated from these codon alignments using the yn00 function of the PAML package (version 4.4; ).
A whole-genome alignment between DH14 and RACE1 was generated using the nucmer and dnadiff functions of the MUMmer software (version 3.9.4; ) with default settings. Alignment gaps (≥1 kb) and inverted regions (≥10 kb) were extracted from the dnadiff 1coords output file. To construct circular visualizations of this alignment, we used the Circos software (version 0.62.1; ). For the overview plot, we initially picked the 8 and 11 largest contigs from the DH14 and RACE1 genomes, based on the corresponding N50 values. For each of these contigs we then extracted any further aligning contigs from the other isolate, for which the sum of all aligned regions (with size ≥2 kb and sequence similarity ≥75%) covered at least 10% of both contigs. For the more detailed view of the large-scale rearrangements, we initially selected the contigs with the observed breakpoints and extracted all aligning contigs from the other isolate, for which the sum of all aligning regions (with size ≥1 kb and sequence similarity ≥75%) covered at least 25% of at least one of the contigs. The circular visualizations also depict gene and TE densities along the genome, which were calculated in 10 kb sliding windows (moving by 1 kb at each step) as fraction of bp within each window that is covered by a gene annotation or TE, respectively. For the linear alignment visualizations of the two largest DH14 contigs, we included all aligning regions of at least 1 kb and plotted the corresponding sequence identities from the MUMmer output together with the corresponding gene and TE densities along those contigs. The detailed view of the local inversions observed within the otherwise syntenic alignment between RACE1 tig00005299 and DH14 scaffold 35 was generated with SyMap (version 4.2; ).
Secretome and core effectorome analysis
The secretomes of all genomes assayed here were identified based on the presence of a signal peptide as detected with SignalP (version 4.1; ) and absence of any transmembrane domain in the mature protein as predicted by TMHMM (version 2.0; ). Functional domain annotation of the proteomes was performed with InterProScan .
To define the core Blumeria-specific effectorome, we assembled the genomes of the formae speciales avenae, dicocci, dactylis, lolii, poae, secalis and triticale using the publicly available raw Illumina reads for the isolates AVE, LIB1609, DAC, LOL, POAE, S1459 and T1–20 (Additional file 1: Table S13). The assemblies were carried out using ABySS 2.0.2 , and the gene space coverage with BUSCO (Additional file 1: Table S14). For the forma specialis tritici the reference assembly of the isolate 96,224 was used. The resulting contig sequences were de novo-annotated with one round of MAKER using the same settings as for the DH14 annotation (described previously, also https://github.com/lambros-f/blumeria_2017).
To remove widely conserved, non-Blumeria specific proteins, all predicted secreted proteins were used as query in BLASTP searches (version 2.5.0+) against the NCBI non-redundant protein database (nr) with the e-value threshold of 10e-5. Additionally, to derive the presence of core Blumeria-specific SPs, an ortholog search was performed using OrthoFinder and the predicted proteomes of the formae speciales. To remove potential bias originating from possible conserved secretion signal peptide sequences, the predicted Bgh SPs were inserted in the analysis as mature peptides.
To generate a maximum likelihood-based phylogenetic tree for the SPs, all the Bgh DH14 mature peptide sequences were aligned with MAFFT v7.310 (−-maxiterate 1000 –localpair; ). Afterwards IQ-TREE multicore version 1.6.beta4  and ModelFinder  were used to select an optimum substitution model and generate the final ML tree. The substitution model used was VT + R8.
To further assess whether SPs or CSEPs are located in gene sparse regions, BEDTools  with the functions complement and closest was utilized to calculate the 5′ and 3′ intergenic space lengths for all genes. The resulting tables were introduced in to R in order to generate the corresponding figure using ggplots2. The corresponding R script is deposited in https://github.com/lambros-f/blumeria_2017. As further control we extracted a set of ascomycete core ortholog genes (COGs) based on the BUSCO Ascomycota odb9 hidden Markov models (http://busco.ezlab.org/datasets/ascomycota_odb9.tar.gz).
Divergence landscapes of transposable elements
To generate divergence landscapes for the TEs of the Letiomycete fungi, repeat elements were identified in all genomes using RepeatMasker (version 4.0.7, http://www.repeatmasker.org/) with default parameters and fungi as the query species based on the Repbase database version 20,150,807 (downloaded on 2016/06/09). Afterwards the RepeatMasker align output (.aln) was parsed using previously described Perl scripts (https://github.com/4ureliek/Parsing-RepeatMasker-Outputs, ). The selection of genomes used for this analysis (Additional file 1: Table S13) and their relation to Bgh was derived from the orthology analysis of their proteomes using OrthoFinder . For the analysis of the dicot-infecting powdery mildews the publicly available assemblies were used (Additional file 1: Table S13), or in the case of G. orontii isolate MGH1 the PacBio reads were assembled with Canu as described previously. It should be noted that proportions of TE types differ in part from previous publications due to usage of the public Repbase database in this work and customized TE libraries in [11, 97].
Duplicate gene search and copy number variation analysis
In order to assess whether duplicate genes exist in the Bgh DH14 and RACE1 genomes, MCScanX was used  with the default parameters. Subsequent analysis to derive copy number variation in all formae speciales and their corresponding isolates was carried out as follows. All genomic reads were first quality trimmed using Trimmomatic (version 0.36; ) and then aligned to the DH14 genome using BWA-MEM . The resulting bam file was sorted using Picard (http://broadinstitute.github.io/picard) and the read depth per bp was extracted using BEDTools . The copy number of each SP was calculated by the average per bp coverage of the gene model by the respective mapped reads, divided by the average coverage of all 805 SPs using custom R scripts. The distance matrix was computed using the Euclidean method, and the heatmap was generated using heatmap.2 from the package gplots. The bash and R scripts used for this analysis can be found in https://github.com/lambros-f/blumeria_2017.
Phylogeny of the isolates
The phylogenetic relationship of the formae speciales and their corresponding isolates was derived from SNPs. The genomic reads of every isolate were mapped to the DH14 reference genome with BWA-MEM , and the GATK best practices pipeline [101, 102] was used for SNP discovery, as previously described . Afterwards, VCFtools 0.1.15  was deployed with the option --max-missing 1 to keep only common SNPs, resulting in 1,070,264 sites. The resulting VCF files were parsed with custom Perl and bash scripts (https://github.com/lambros-f/blumeria_2017) and imported to SplitsTree  to generate a cladogram based on an UPGMA tree.
For isolates A6 and K1, SNPs to DH14 were identified with GATK [101, 102] from the BWA-MEM  alignment of short sequence reads as described above. For RACE1, SNPs to DH14 were identified using the nucmer and dnadiff functions of the MUMmer software (version 3.9.4; ) with default settings. Subsequently, for all three isolates, we calculated the SNP frequency as a function of the genomic location by using a 10 kb sliding window that moved 1 kb at each step for all DH14 contigs larger than 50 kb. To further examine the distribution of low and high SNP frequencies, we applied the expectation-maximization (EM) algorithm (function normalmixEM, R-package mixtools) to fit a two-component mixture model to the observed SNP frequencies as described previously [12, 19].
- AVR :
Avirulence effector gene
- Bgh :
Blumeria graminis f.sp. hordei
Copy number variation
Candidate secreted effector protein
Expressed sequence tag
Fragments per kilobase [sequence length] and million [sequenced fragments]
Single nucleotide polymorphism
Glawe DA. The powdery mildews: a review of the world's most familiar (yet poorly known) plant pathogens. Annu Rev Phytopathol. 2008;46:27–51. https://doi.org/10.1146/annurev.phyto.46.081407.104740.
Kuhn H, Kwaaitaal M, Kusch S, Acevedo-Garcia J, Wu H, Panstruga R. Biotrophy at its best: novel findings and unsolved mysteries of the Arabidopsis-powdery mildew pathosystem. The Arabidopsis Book. 2016;14:e0184. https://doi.org/10.1199/tab.0184.
Lipka U, Fuchs R, Lipka V. Arabidopsis non-host resistance to powdery mildews. Curr Opin Plant Biol. 2008;11:404–11. https://doi.org/10.1016/j.pbi.2008.04.004.
Kusch S, Panstruga R. mlo-based resistance: an apparently universal “weapon” to defeat powdery mildew disease. Mol Plant-Microbe Interact. 2017;30:179–89. https://doi.org/10.1094/MPMI-12-16-0255-CR.
Tucker MA, Lopez-Ruiz F, Jayasena K, Oliver RP. Origin of fungicide-resistant barley powdery mildew in Western Australia: lessons to be learned. In: Ishii H, Hollomon DW, editors. Fungicide resistance in plant pathogens: principles and a guide to practical management. Tokyo: Springer; 2015. p. 329–40. https://doi.org/10.1007/978-4-431-55642-8_20.
Jones L, Riaz S, Morales-Cruz A, Amrine KCH, McGuire B, Gubler WD, et al. Adaptive genomic structural variation in the grape powdery mildew pathogen, Erysiphe necator. BMC Genomics. 2014;15:1081. https://doi.org/10.1186/1471-2164-15-1081.
Brown JKM. Durable resistance of crops to disease: a Darwinian perspective. Annu Rev Phytopathol. 2015;53:513–39. https://doi.org/10.1146/annurev-phyto-102313-045914.
Wyand RA, Brown JKM. Genetic and forma specialis diversity in Blumeria graminis of cereals and its implications for host-pathogen co-evolution. Mol Plant Pathol. 2003;4:187–98. https://doi.org/10.1046/j.1364-3703.2003.00167.x.
Lu X, Kracher B, Saur IML, Bauer S, Ellwood SR, Wise R, et al. Allelic barley MLA immune receptors recognize sequence-unrelated avirulence effectors of the powdery mildew pathogen. Proc Natl Acad Sci U S A. 2016;113:E6486–95. https://doi.org/10.1073/pnas.1612947113.
Bindschedler LV, Panstruga R, Spanu PD. Mildew-omics: how global analyses aid the understanding of life and evolution of powdery mildews. Front Plant Sci. 2016;7:123. https://doi.org/10.3389/fpls.2016.00123.
Spanu PD, Abbott JC, Amselem J, Burgis TA, Soanes DM, Stüber K, et al. Genome expansion and gene loss in powdery mildew fungi reveal tradeoffs in extreme parasitism. Science. 2010;330:1543–6.
Wicker T, Oberhaensli S, Parlange F, Buchmann JP, Shatalina M, Roffler S, et al. The wheat powdery mildew genome shows the unique evolution of an obligate biotroph. Nat Genet. 2013;45:1092–6. https://doi.org/10.1038/ng.2704.
Pedersen C, Ver Loren van Themaat E, LJ MG, Abbott JC, Burgis TA, Barton G, et al. Structure and evolution of barley powdery mildew effector candidates. BMC Genomics. 2012;13:694. https://doi.org/10.1186/1471-2164-13-694.
Bourras S, McNally KE, Müller MC, Wicker T, Keller B. Avirulence genes in cereal powdery mildews: the gene-for-gene hypothesis 2.0. Front. Plant Sci. 2016;7:241. https://doi.org/10.3389/fpls.2016.00241.
Praz CR, Bourras S, Zeng F, Sánchez-Martín J, Menardo F, Xue M, et al. AvrPm2 encodes an RNase-like avirulence effector which is conserved in the two different specialized forms of wheat and rye powdery mildew fungus. New Phytol. 2017;213:1301–14. https://doi.org/10.1111/nph.14372.
Menardo F, Praz CR, Wyder S, Ben-David R, Bourras S, Matsumae H, et al. Hybridization of powdery mildew strains gives rise to pathogens on novel agricultural crop species. Nat Genet. 2016;48:201–5. https://doi.org/10.1038/ng.3485.
Troch V, Audenaert K, Bekaert B, Höfte M, Haesaert G. Phylogeography and virulence structure of the powdery mildew population on its ‘new’ host triticale. BMC Evol Biol. 2012;12:76. https://doi.org/10.1186/1471-2148-12-76.
Menardo F, Wicker T, Keller B. Reconstructing the evolutionary history of powdery mildew lineages (Blumeria graminis) at different evolutionary time scales with NGS data. Genome Biol Evol. 2017;9:446–56. https://doi.org/10.1093/gbe/evx008.
Hacquard S, Kracher B, Maekawa T, Vernaldi S, Schulze-Lefert P, Ver Loren van Themaat E. Mosaic genome structure of the barley powdery mildew pathogen and conservation of transcriptional programs in divergent hosts. Proc Natl Acad Sci U S A. 2013;110:28. https://doi.org/10.1073/pnas.1306807110.
Koren S, Walenz BP, Berlin K, Miller JR, Bergman NH, Phillippy AM. Canu: scalable and accurate long-read assembly via adaptive k-mer weighting and repeat separation. Genome Res. 2017;27:722–36. https://doi.org/10.1101/gr.215087.116.
Giese H, Christiansen SK, Jensen HP. Extrachromosomal plasmid-like DNA in the obligate parasitic fungus Erysiphe graminis f.Sp. hordei. Theor Appl Genet. 1990;79:56–64.
Pedersen C, Rasmussen SW, Giese H. A genetic map of Blumeria graminis based on functional genes, avirulence genes, and molecular markers. Fungal Genet Biol. 2002;35:235–46.
Borbye L, Linde-Laursen I, Christiansen SK, Giese H. The chromosome complement of Erysiphe graminis f.Sp. hordei analysed by light microscopy and field inversion gel electrophoresis. Mycol Res. 1992;96:97–102. https://doi.org/10.1016/S0953-7562(09)80922-2.
Robinson HL, Ridout CJ, Sierotzki H, Gisi U, Brown JKM. Isogamous, hermaphroditic inheritance of mitochondrion-encoded resistance to Qo inhibitor fungicides in Blumeria graminis f. Sp. tritici. Fungal Genet Biol. 2002;36:98–106. https://doi.org/10.1016/S1087-1845(02)00006-3.
Mardanov AV, Beletsky AV, Kadnikov VV, Ignatov AN, Ravin NV. The 203 kbp mitochondrial genome of the phytopathogenic fungus Sclerotinia borealis reveals multiple invasions of introns and genomic duplications. PLoS One. 2014;9:e107536. https://doi.org/10.1371/journal.pone.0107536.
Bietenhader M, Martos A, Tetaud E, Aiyar RS, Sellem CH, Kucharczyk R, et al. Experimental relocation of the mitochondrial ATP9 gene to the nucleus reveals forces underlying mitochondrial genome evolution. PLoS Genet. 2012;8:e1002876. https://doi.org/10.1371/journal.pgen.1002876.
Déquard-Chablat M, Sellem CH, Golik P, Bidard F, Martos A, Bietenhader M, et al. Two nuclear life cycle-regulated genes encode interchangeable subunits c of mitochondrial ATP synthase in Podospora anserina. Mol Biol Evol. 2011;28:2063–75. https://doi.org/10.1093/molbev/msr025.
Campbell MS, Holt C, Moore B, Yandell M. Genome annotation and curation using MAKER and MAKER-P. Curr Protoc Bioinformatics. 2014;48:4.11.1–39. https://doi.org/10.1002/0471250953.bi0411s48.
Kusch S, Ahmadinejad N, Panstruga R, Kuhn H. In silico analysis of the core signaling proteome from the barley powdery mildew pathogen (Blumeria graminis f.Sp. hordei). BMC Genomics. 2014;15:843. https://doi.org/10.1186/1471-2164-15-843.
Robinson JT, Thorvaldsdóttir H, Winckler W, Guttman M, Lander ES, Getz G, Mesirov JP. Integrative genomics viewer. Nat Biotechnol. 2011;29:24–6. https://doi.org/10.1038/nbt.1754.
Kurtz S, Phillippy A, Delcher AL, Smoot M, Shumway M, Antonescu C, Salzberg SL. Versatile and open software for comparing large genomes. Genome Biol. 2004;5:R12. https://doi.org/10.1186/gb-2004-5-2-r12.
Wang Y, Li J, Paterson AH. MCScanX-transposed: detecting transposed gene duplications based on multiple colinearity scans. Bioinformatics. 2013;29:1458–60. https://doi.org/10.1093/bioinformatics/btt150.
Rouxel T, Grandaubert J, Hane JK, Hoede C, van de Wouw AP, Couloux A, et al. Effector diversification within compartments of the Leptosphaeria maculans genome affected by repeat-induced point mutations. Nat Commun. 2011;2:202. https://doi.org/10.1038/ncomms1189.
Klosterman SJ, Subbarao KV, Kang S, Veronese P, Gold SE, Thomma BPHJ, et al. Comparative genomics yields insights into niche adaptation of plant vascular wilt pathogens. PLoS Pathog. 2011;7:e1002137. https://doi.org/10.1371/journal.ppat.1002137.
Takamatsu S, Matsuda S. Estimation of molecular clocks for ITS and 28S rDNA in Erysiphales. Mycoscience. 2004;45:340–4.
Mori Y, Sato Y, Takamatsu S. Molecular phylogeny and radiation time of the Erysiphales inferred from the nuclear ribosomal DNA sequences. Mycoscience. 2000;41:437–47.
Haas BJ, Kamoun S, Zody MC, Jiang RHY, Handsaker RE, Cano LM, et al. Genome sequence and analysis of the Irish potato famine pathogen Phytophthora infestans. Nature. 2009;461:393–8.
Castanera R, López-Varas L, Borgognone A, LaButti K, Lapidus A, Schmutz J, et al. Transposable elements versus the fungal genome: impact on whole-genome architecture and transcriptional profiles. PLoS Genet. 2016;12:e1006108. https://doi.org/10.1371/journal.pgen.1006108.
Lo Presti L, Lanver D, Schweizer G, Tanaka S, Liang L, Tollot M, et al. Fungal effectors and plant susceptibility. Annu Rev Plant Biol. 2015;66:513–45. https://doi.org/10.1146/annurev-arplant-043014-114623.
Cheng C, Dong Z, Han X, Wang H, Jiang L, Sun J, et al. Thioredoxin a is essential for motility and contributes to host infection of Listeria monocytogenes via redox interactions. Front Cell Infect Microbiol. 2017;7:287. https://doi.org/10.3389/fcimb.2017.00287.
Cintra LC, Domingos FC, Lima YAR, Barbosa MS, Santos RS, Faria FP, Jesuíno RSA. Molecular cloning, expression and insulin reduction activity of a thioredoxin 1 homologue (TRX1) from the pathogenic fungus Paracoccidioides lutzii. Int J Biol Macromol. 2017;103:683–91. https://doi.org/10.1016/j.ijbiomac.2017.05.114.
Faino L, Seidl MF, Shi-Kunne X, Pauper M, van den Berg GCM, Wittenberg AHJ, Thomma BPHJ. Transposons passively and actively contribute to evolution of the two-speed genome of a fungal pathogen. Genome Res. 2016;26:1091–100. https://doi.org/10.1101/gr.204974.116.
de Jonge R, Bolton MD, Kombrink A, van den Berg GCM, Yadeta KA, Thomma BPHJ. Extensive chromosomal reshuffling drives evolution of virulence in an asexual pathogen. Genome Res. 2013;23:1271–82. https://doi.org/10.1101/gr.152660.112.
Dong S, Raffaele S, Kamoun S. The two-speed genomes of filamentous pathogens: waltz with plants. Curr Opin Plant Biol. 2015;35:57–65. https://doi.org/10.1016/j.gde.2015.09.001.
Yoshida K, Saunders DGO, Mitsuoka C, Natsume S, Kosugi S, Saitoh H, et al. Host specialization of the blast fungus Magnaporthe oryzae is associated with dynamic gain and loss of genes linked to transposable elements. BMC Genomics. 2016;17:370. https://doi.org/10.1186/s12864-016-2690-6.
Wit PJGM de, Testa AC, Oliver RP. Fungal plant pathogenesis mediated by effectors. Microbiol Spectr. 2016. doi:https://doi.org/10.1128/microbiolspec.FUNK-0021-2016.
Inoue Y, Vy TTP, Yoshida K, Asano H, Mitsuoka C, Asuke S, et al. Evolution of the wheat blast fungus through functional losses in a host specificity determinant. Science. 2017;357:80–3. https://doi.org/10.1126/science.aam9654.
Ma LJ, van der Does HC, Borkovich KA, Coleman JJ, Daboussi MJ, Di Pietro A, et al. Comparative genomics reveals mobile pathogenicity chromosomes in Fusarium. Nature. 2010;464:367–73.
Hartmann FE, Sánchez-Vallet A, McDonald BA, Croll D. A fungal wheat pathogen evolved host specialization by extensive chromosomal rearrangements. ISME J. 2017;11:1189–204. https://doi.org/10.1038/ismej.2016.196.
Chiapello H, Mallet L, Guérin C, Aguileta G, Amselem J, Kroj T, et al. Deciphering genome content and evolutionary relationships of isolates from the fungus Magnaporthe oryzae attacking different host plants. Genome Biol Evol. 2015;7:2896–912. https://doi.org/10.1093/gbe/evv187.
Manning VA, Pandelova I, Dhillon B, Wilhelm LJ, Goodwin SB, Berlin AM, et al. Comparative genomics of a plant-pathogenic fungus, Pyrenophora tritici-repentis, reveals transduplication and the impact of repeat elements on pathogenicity and population divergence. G3. 2013;3:41–63. https://doi.org/10.1534/g3.112.004044.
Martinez JP, Oesch NW, Ciuffetti LM. Characterization of the multiple-copy host-selective toxin gene, ToxB, in pathogenic and nonpathogenic isolates of Pyrenophora tritici-repentis. Mol Plant-Microbe Interact. 2004;17:467–74. https://doi.org/10.1094/MPMI.2004.17.5.467.
Freitag M, Williams RL, Kothe GO, Selker EU. A cytosine methyltransferase homologue is essential for repeat-induced point mutation in Neurospora crassa. Proc Natl Acad Sci U S A. 2002;99:8802–7. https://doi.org/10.1073/pnas.132212899.
Menardo F, Praz CR, Wicker T, Keller B. Rapid turnover of effectors in grass powdery mildew (Blumeria graminis). BMC Evol Biol. 2017;17:223. https://doi.org/10.1186/s12862-017-1064-2.
Raffaele S, Kamoun S. Genome evolution in filamentous plant pathogens: why bigger can be better. Nat Rev Microbiol. 2012;10:417–30. https://doi.org/10.1038/nrmicro2790.
Rasmussen M, Rossen L, Giese H. SINE-like properties of a highly repetitive element in the genome of the obligate parasitic fungus Erysiphe graminis f.sp. hordei. Mol Gen Genet. 1993;239:298–303.
Wei YD, Collinge DB, Smedegaard-Petersen V, Thordal-Christensen H. Characterization of the transcript of a new class of retroposon-type repetitive element cloned from the powdery mildew fungus, Erysiphe graminis. Mol Gen Genet. 1996;250:477–82.
Oberhaensli S, Parlange F, Buchmann JP, Jenny FH, Abbott JC, Burgis TA, et al. Comparative sequence analysis of wheat and barley powdery mildew fungi reveals gene colinearity, dates divergence and indicates host-pathogen co-evolution. Fungal Genet Biol. 2011;48:327–34. https://doi.org/10.1016/j.fgb.2010.10.003.
Kang S, Lebrun MH, Farrall L, Valent B. Gain of virulence caused by insertion of a Pot3 transposon in a Magnaporthe grisea avirulence gene. Mol Plant-Microbe Interact. 2001;14:671–4. https://doi.org/10.1094/MPMI.2001.14.5.671.
Ali S, Laurie JD, Linning R, Cervantes-Chávez JA, Gaudet D, Bakkeren G. An immunity-triggering effector from the barley smut fungus Ustilago hordei resides in an Ustilaginaceae-specific cluster bearing signs of transposable element-assisted evolution. PLoS Pathog. 2014;10:e1004223. https://doi.org/10.1371/journal.ppat.1004223.
Grandaubert J, Lowe RG, Soyer JL, Schoch CL, van de Wouw AP, Fudal I, et al. Transposable element-assisted evolution and adaptation to host plant within the Leptosphaeria maculans-Leptosphaeria biglobosa species complex of fungal pathogens. BMC Genomics. 2014;15:891. https://doi.org/10.1186/1471-2164-15-891.
Rebollo R, Horard B, Hubert B, Vieira C. Jumping genes and epigenetics: towards new species. Gene. 2010;454:1–7. https://doi.org/10.1016/j.gene.2010.01.003.
Startek M, Le Rouzic A, Capy P, Grzebelus D, Gambin A. Genomic parasites or symbionts? Modeling the effects of environmental pressure on transposition activity in asexual populations. Theor Popul Biol. 2013;90:145–51. https://doi.org/10.1016/j.tpb.2013.07.004.
McFadden J, Knowles G. Escape from evolutionary stasis by transposon-mediated deleterious mutations. J Theor Biol. 1997;186:441–7. https://doi.org/10.1006/jtbi.1997.0403.
Feehan JM, Scheibel KE, Bourras S, Underwood W, Keller B, Somerville SC. Purification of high molecular weight genomic DNA from powdery mildew for long-read sequencing. J Vis Exp. 2017. doi:https://doi.org/10.3791/55463.
Eid J, Fehr A, Gray J, Luong K, Lyle J, Otto G, et al. Real-time DNA sequencing from single polymerase molecules. Science. 2009;323:133–8. https://doi.org/10.1126/science.1162986.
Chin C-S, Alexander DH, Marks P, Klammer AA, Drake J, Heiner C, et al. Nonhybrid, finished microbial genome assemblies from long-read SMRT sequencing data. Nat Methods. 2013;10:563–9. https://doi.org/10.1038/nmeth.2474.
Sahlin K, Vezzi F, Nystedt B, Lundeberg J, Arvestad L. BESST- efficient scaffolding of large fragmented assemblies. BMC Bioinformatics. 2014;15:281. https://doi.org/10.1186/1471-2105-15-281.
Walker BJ, Abeel T, Shea T, Priest M, Abouelliel A, Sakthikumar S, et al. Pilon: an integrated tool for comprehensive microbial variant detection and genome assembly improvement. PLoS One. 2014;9:e112963. https://doi.org/10.1371/journal.pone.0112963.
Simão FA, Waterhouse RM, Ioannidis P, Kriventseva EV, Zdobnov EM. BUSCO: assessing genome assembly and annotation completeness with single-copy orthologs. Bioinformatics. 2015;31:3210–2. https://doi.org/10.1093/bioinformatics/btv351.
Camacho C, Coulouris G, Avagyan V, Ma N, Papadopoulos J, Bealer K, Madden TL. BLAST+: architecture and applications. BMC Bioinformatics. 2009;10:421. https://doi.org/10.1186/1471-2105-10-421.
Kim D, Pertea G, Trapnell C, Pimentel H, Kelley R, Salzberg SL. TopHat2: accurate alignment of transcriptomes in the presence of insertions, deletions and gene fusions. Genome Biol. 2013;14:R36. https://doi.org/10.1186/gb-2013-14-4-r36.
Liao Y, Smyth GK, Shi W. featureCounts: an efficient general purpose program for assigning sequence reads to genomic features. Bioinformatics. 2014;30:923–30. https://doi.org/10.1093/bioinformatics/btt656.
Dobin A, Davis CA, Schlesinger F, Drenkow J, Zaleski C, Jha S, et al. STAR: Ultrafast universal RNA-seq aligner. Bioinformatics. 2013;29:15–21. https://doi.org/10.1093/bioinformatics/bts635.
Holt C, Yandell M. MAKER2: an annotation pipeline and genome-database management tool for second-generation genome projects. BMC Bioinformatics. 2011;12:491. https://doi.org/10.1186/1471-2105-12-491.
Haas BJ, Papanicolaou A, Yassour M, Grabherr M, Blood PD, Bowden J, et al. De novo transcript sequence reconstruction from RNA-seq using the trinity platform for reference generation and analysis. Nat Protoc. 2013;8:1494–512. https://doi.org/10.1038/nprot.2013.084.
Stanke M, Keller O, Gunduz I, Hayes A, Waack S, Morgenstern B. AUGUSTUS: Ab initio prediction of alternative transcripts. Nucleic Acids Res. 2006;34:W435–9. https://doi.org/10.1093/nar/gkl200.
Korf I. Gene finding in novel genomes. BMC Bioinformatics. 2004;5:59. https://doi.org/10.1186/1471-2105-5-59.
Ter-Hovhannisyan V, Lomsadze A, Chernoff YO, Borodovsky M. Gene prediction in novel fungal genomes using an ab initio algorithm with unsupervised training. Genome Res. 2008;18:1979–90. https://doi.org/10.1101/gr.081612.108.
Lee E, Helt GA, Reese JT, Munoz-Torres MC, Childers CP, Buels RM, et al. Web Apollo: a web-based genomic annotation editing platform. Genome Biol. 2013;14:R93. https://doi.org/10.1186/gb-2013-14-8-r93.
Slater GSC, Birney E. Automated generation of heuristics for biological sequence comparison. BMC Bioinformatics. 2005;6:31. https://doi.org/10.1186/1471-2105-6-31.
Emms DM, Kelly S. OrthoFinder: solving fundamental biases in whole genome comparisons dramatically improves orthogroup inference accuracy. Genome Biol. 2015;16:157. https://doi.org/10.1186/s13059-015-0721-2.
Larkin MA, Blackshields G, Brown NP, Chenna R, McGettigan PA, McWilliam H, et al. Clustal W and Clustal X version 2.0. Bioinformatics. 2007;23:2947–8. https://doi.org/10.1093/bioinformatics/btm404.
Suyama M, Torrents D, Bork P. PAL2NAL: robust conversion of protein sequence alignments into the corresponding codon alignments. Nucleic Acids Res. 2006;34:W609–12. https://doi.org/10.1093/nar/gkl315.
Yang Z. PAML 4: phylogenetic analysis by maximum likelihood. Mol Biol Evol. 2007;24:1586–91. https://doi.org/10.1093/molbev/msm088.
Krzywinski M, Schein J, Birol I, Connors J, Gascoyne R, Horsman D, et al. Circos: an information aesthetic for comparative genomics. Genome Res. 2009;19:1639–45. https://doi.org/10.1101/gr.092759.109.
Soderlund C, Bomhoff M, Nelson WM. SyMAP v3.4: a turnkey synteny system with application to plant genomes. Nucleic Acids Res. 2011;39:e68. https://doi.org/10.1093/nar/gkr123.
Petersen TN, Brunak S, von Heijne G, Nielsen H. SignalP 4.0: discriminating signal peptides from transmembrane regions. Nat Methods. 2011;8:785–6. https://doi.org/10.1038/nmeth.1701.
Emanuelsson O, Brunak S, von Heijne G, Nielsen H. Locating proteins in the cell using TargetP, SignalP and related tools. Nat Protoc. 2007;2:953–71. https://doi.org/10.1038/nprot.2007.131.
Jones P, Binns D, Chang H-Y, Fraser M, Li W, McAnulla C, et al. InterProScan 5: genome-scale protein function classification. Bioinformatics. 2014;30:1236–40. https://doi.org/10.1093/bioinformatics/btu031.
Jackman SD, Vandervalk BP, Mohamadi H, Chu J, Yeo S, Hammond SA, et al. ABySS 2.0: resource-efficient assembly of large genomes using a bloom filter. Genome Res. 2017;27:768–77. https://doi.org/10.1101/gr.214346.116.
Katoh K, Standley DM. MAFFT multiple sequence alignment software version 7: improvements in performance and usability. Mol Biol Evol. 2013;30:772–80. https://doi.org/10.1093/molbev/mst010.
Chernomor O, von Haeseler A, Minh BQ. Terrace aware data structure for phylogenomic inference from supermatrices. Syst Biol. 2016;65:997–1008. https://doi.org/10.1093/sysbio/syw037.
Kalyaanamoorthy S, Minh BQ, Wong TKF, von Haeseler A, Jermiin LS. ModelFinder: fast model selection for accurate phylogenetic estimates. Nat Methods. 2017;14:587–9. https://doi.org/10.1038/nmeth.4285.
Quinlan AR, Hall IM. BEDTools: a flexible suite of utilities for comparing genomic features. Bioinformatics. 2010;26:841–2. https://doi.org/10.1093/bioinformatics/btq033.
Kapusta A, Suh A, Feschotte C. Dynamics of genome size evolution in birds and mammals. Proc Natl Acad Sci U S A. 2017;114:E1460–9. https://doi.org/10.1073/pnas.1616702114.
Amselem J, Vigouroux M, Oberhaensli S, Brown JKM, Bindschedler LV, Skamnioti P, et al. Evolution of the EKA family of powdery mildew avirulence-effector genes from the ORF 1 of a LINE retrotransposon. BMC Genomics. 2015;16:917. https://doi.org/10.1186/s12864-015-2185-x.
Bolger AM, Lohse M, Usadel B. Trimmomatic: a flexible trimmer for Illumina sequence data. Bioinformatics. 2014;30:2114–20. https://doi.org/10.1093/bioinformatics/btu170.
Li H, Durbin R. Fast and accurate short read alignment with burrows-wheeler transform. Bioinformatics. 2009;25:1754–60. https://doi.org/10.1093/bioinformatics/btp324.
Li H. Aligning sequence reads, clone sequences and assembly contigs with BWA-MEM. https://arxiv.org/abs/1303.3997. Accessed 28 Oct 2017.
DePristo MA, Banks E, Poplin R, Garimella KV, Maguire JR, Hartl C, et al. A framework for variation discovery and genotyping using next-generation DNA sequencing data. Nat Genet. 2011;43:491–8. https://doi.org/10.1038/ng.806.
McKenna A, Hanna M, Banks E, Sivachenko A, Cibulskis K, Kernytsky A, et al. The genome analysis toolkit: a MapReduce framework for analyzing next-generation DNA sequencing data. Genome Res. 2010;20:1297–303. https://doi.org/10.1101/gr.107524.110.
Islam MT, Croll D, Gladieux P, Soanes DM, Persoons A, Bhattacharjee P, et al. Emergence of wheat blast in Bangladesh was caused by a south American lineage of Magnaporthe oryzae. BMC Biol. 2016;14:84. https://doi.org/10.1186/s12915-016-0309-7.
Danecek P, Auton A, Abecasis G, Albers CA, Banks E, DePristo MA, et al. The variant call format and VCFtools. Bioinformatics. 2011;27:2156–8. https://doi.org/10.1093/bioinformatics/btr330.
Huson DH, Bryant D. Application of phylogenetic networks in evolutionary studies. Mol Biol Evol. 2006;23:254–67. https://doi.org/10.1093/molbev/msj030.
Rice P, Longden I, Bleasby A. EMBOSS: the European molecular biology open software suite. Trends Genet. 2000;16:276–7.
Huson DH, Richter DC, Rausch C, Dezulian T, Franz M, Rupp R. Dendroscope: an interactive viewer for large phylogenetic trees. BMC Bioinformatics. 2007;8:460. https://doi.org/10.1186/1471-2105-8-460.
We would like to acknowledge the help of Helder Pedro and of the PhytoPathDB (http://www.phytopathdb.org/) for supporting the re-annotation of the reference isolate DH14. The analysis was performed with computing resources granted by RWTH Aachen University under project rwth0146.
This work was supported by a grant of the Deutsche Forschungsgemeinschaft (DFG)-funded Priority Programme SPP1819 (Rapid evolutionary adaptation - Potential and constraints) to R.P. (PA 861/14–1), the DFG-funded Collaborative Research Centre SFB670/3 (Cell-autonomous Immunity) to P.S.L. (grant #13123509) and the Danish Strategic Research Council (grant no. 10-093504) to C.P.
Availability of data and materials
The genome sequencing and assembly data generated in this study have been deposited under the ENA Project IDs PRJEB23502 and PRJEB23162. The new assembly and annotation for the reference Blumeria graminis f.sp. hordei DH14 genome is in addition available through the PhytopathDB database (http://fungi.ensembl.org/Blumeria_graminis/Info/Index). The RNA-seq data for DH14 generated in this study has been deposited in the Gene Expression Omnibus (GEO) database, www.ncbi.nlm.nih.gov/geo (accession no. GSE106282).
Ethics approval and consent to participate
The authors declare that they have no competing interests.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Table S1. BUSCO genome completeness analysis. Table S2. Scaffolds with telomeric repeats at their ends in the DH14 and RACE1 assembly. Table S3. Assosiation table for old and new Bgh gene model IDs. Table S4. Manually currated orthology relationships between RACE1 and DH14. Table S5. Isolate-specific genes in DH14 and RACE1. Table S6. Isolate-specific gene expression in DH14 and RACE1. Table S7. Clustering of secreted protein coding genes in the Bgh DH14 genome. Table S8. MCScanX analysis for the identification of duplicate genes. Table S9. Functional domains of dispersed duplicate genes in Sclerotinia sclerotiorum. Table S10. Secreted/Non-secreted duplications in the Bgh DH14 genome. Table S12. Raw read count for the top 20 expressing transposable elements in pooled 16 h & 48 h dpi DH14 RNA-seq dataset. Table S13. All datasets used for analyses in this study. Table S14. BUSCO analysis for the forma specialis genomes used for orthology calling between the CSEPs. (XLSX 1151 kb)
Figure S1. Comparative alignment of the Bgh DH14 and RACE1 genome assemblies with a Bgh genetic map. The distribution and ordering of 80 single copy EST markers across 30 linkage groups of a previously published genetic map  is visualized in relation to the corresponding genomic locations of these markers in the DH14/RACE1 assemblies. Each box represents a specific genomic contig or linkage group (LG), respectively, and the numbers inside the boxes specify the marker positions on the corresponding contig (in bp) or linkage group (in cM). The corresponding marker identifiers are given next to the boxes. Dashed connector lines represent markers for which the genomic location and genetic map are consistent. Discrepancies between assembly and genetic map are indicated by solid connectors, with black lines representing markers whose location is consistent between assemblies but different from the genetic map, and colored lines representing markers with differences to the genetic map that are specific to either DH14 (dark pink) or RACE1 (blue). (PDF 4159 kb)
Figure S2. Involvement of TEs in chromosomal organization. (A) Density of different categories of repetitive elements and genes per 50 kb sliding windows in selected scaffolds with putative centromeric regions. A subset of Tad1-like LINE elements that are associated with putative centromeric regions are highlighted in green. (B) Box plots of the 5′ and 3′ intergenic distances for ascomycete core ortholog genes (COGs), CSEPs and other secreted protein-coding genes that do not fulfil the CSEP criteria (“other SPs”). No statistically significant differences were detected for the 5′ distances (p = 0.382; ANOVA) and differing letters indicate statistically significant differences between groups for the 3′ distances (p < 0.05; ANOVA with Tukey post hoc tests). (C) Plots depicting by color-code the dN/dS ratio of each gene of the three different groups (COGs, CSEPs, other SPs) in relation to their flanking intergenic length. Genes with dS values of 0 are not shown. (PDF 1888 kb)
Figure S3. Mitochondrial genomes of Bgh. (A) Map and corresponding annotation of the mitochondrial genome of Bgh isolate DH14 resulting from an RNAweasel and MFannot run. (B) Nucleotide sequence alignment between the DH14 (x-axis) and RACE1 (y-axis) mtDNA using NUCmer, indicating a putative partial duplication in RACE1. (PDF 224 kb)
Figure S4. Comparative visualization of the genomic loci harboring AVR a1 and AVR a13 in the Bgh isolates DH14 and RACE1. (A) Organization of the genomic locus harboring the previously identified AVR a1 (orange arrows) and some of its flanking genes in DH14 and RACE1. (B) Organization of the genomic locus harboring the previously identified AVR a13 (green arrows) and some of its flanking genes in DH14 and RACE1. (PDF 1206 kb)
Figure S5. Variation in the mating type locus in the Bgh isolates DH14 and RACE1. Organization of the genomic loci containing the mating type genes (MAT-1-1-1, MAT-1-1-3 and MAT-1-2-1) and some of its flanking genes. As DH14 and RACE1 are of opposite mating types, the structure of the mating type locus differs between the two isolates. The genomic locus in RACE1, which is of the MAT-1-1 mating type, was assembled completely, while the respective locus in DH14 (MAT-1-2 mating type) is distributed on two scaffolds. (PDF 1139 kb)
Figure S6. Evidence for two large-scale genomic rearrangements between the isolates DH14 and RACE1. Circos diagram showing evidence for large-scale genomic rearrangements between DH14 and RACE1. The two scaffolds/contigs in the assemblies of DH14 and RACE1 with internal alignment breaks and the corresponding aligning scaffolds/contigs in the other isolate were extracted for visualization. Syntenic regions and alignment breaks were identified based on a whole-genome alignment, and aligning regions of at least 1 kb between the two isolates (with nucleotide sequence similarity ≥75%) are connected with lines in the circular plot. Lines within the syntenic blocks directly flanking the breaks are shown in color while lines in all other blocks are depicted in grey. The positions of the observed alignment breaks are marked by arrowheads colored in green (three breaks likely involved in the same event) and brown (two breaks likely involved in the same event). The surrounding circles represent from the outside: on the right side the DH14 scaffolds (pink) and on the left side the RACE1 (blue), with all unaligned regions (≥ 0.5 kb) indicated as white gaps on the scaffolds/contigs; the gene density (green) and TE density (blue) calculated in 10 kb sliding windows; the locations of all genes predicted to code for SPs; the locations of isolate-specific genes coding for SPs (dark red) or any other proteins (black); and isolate-specific additional gene copies/paralogs coding for SPs (pink) or any other proteins (grey). (PDF 1023 kb)
Figure S7. Frequency of single-nucleotide polymorphisms (SNPs) between Bgh isolates. (A) Kernel density plot of the SNP frequencies per kb in 10 kb sliding windows, observed for the three Bgh isolates A6, K1 and RACE1 relative to the reference isolate DH14. The plot depicts Gaussian kernel density estimates calculated at a smoothing bandwidth of 0.12. (B) Average SNP frequencies for A6, K1 and RACE1 in 10 kb sliding windows of low and high SNP density as estimated by a two-component mixture model that was fitted to the observed SNP frequencies using the expectation-maximization algorithm. Error bars indicate the corresponding standard deviations estimated by the mixture model. (PDF 294 kb)
Figure S8. Distribution of SP and non-SP coding genes in Bgh DH14 scaffolds larger than 1 MB. (A) Density plots of SP coding genes (orange), non-SP coding genes (purple) and different types of TE elements (gray) in 50 kb sliding windows. Scaffolds depicted here were selected based on their size (> 1 MB) and represent ~ 87% of the total genomic sequence. (B) Number of SP coding genes per scaffold plotted against the respective total scaffold size, showing positive correlation (r = 0.88, p < 0.001). (PDF 4282 kb)
Figure S9. CNV of widely conserved genes between B. graminis formae speciales. Heatmap illustrating the copy number of genes with putatively widely conserved functions. Using the same pipeline as for the generation of Fig. 3a, all 34 genes with a PFAM annotation including the terms “tubulin” (highlighted in red) or “actin” (highlighted in green) and 49 genes coding for non-SP genes with conserved domains were used as a control dataset to estimate the error rate of the CNV calling pipeline. The heatmap depicts the color-coded copy number of these genes per individual genome of various B. graminis formae speciales (avenae, dactylis, dicocci, hordei, lolii, poae, secalis, triticale and tritici), each represented by one or more isolates as indicated on the right. The dendrogram on the left is based on the hierarchical clustering (Euclidean method) of the CNV values for every dataset. (PDF 466 kb)
Figure S10. Secretome orthology relations and core effectorome phylogeny. (A) Heatmap of SP orthologs found for the formae speciales genomes after ortholog clustering using OrthoFinder on the predicted proteomes of the isolates T1–20, S1459, LIB1609, DAC, 96224, LOL, AVE, POAE, DH14. Every column corresponds to one of the 805 Bgh DH14 predicted SPs, while color-coding depicts the number of orthologs in the corresponding orthogroup. Hierarchical clustering (Euclidean method) for the formae speciales and the SPs are given on the left and the top of the heatmap, respectively. (B) Maximum likelihood phylogeny tree of the 805 SPs. The tree was generated using IQ-TREE based on the mature peptide sequences of the Bgh DH14 SPs. Orange edge tips indicate the 190 core CSEPs which have orthologs in all formae speciales. The scale bar indicates the number of amino-acid substitutions per site. (PDF 2195 kb)
Figure S11. Representatives of the genus Blumeria show less TE divergence than representatives of the genera Erishyphe and Golovinomyces. (A) The histograms indicate the frequency of a given sequence divergence for TE families of 10 B. graminis genomes. The genomes, which were assembled based on various sequencing platforms (PacBio or Illumina), were surveyed for their repeat content and repeat landscapes for each genome based on % nucleotide divergence to the consensus TE sequences were calculated out of the RepeatMasker output using Perl scripts. Sequence divergence (x-axis) is plotted against frequency (number of sequences; y-axis) for each of the genomes. (B) The histograms indicate the frequency of a given sequence divergence for TE families of 3 dicot-infecting powdery mildew species (Erysiphe pisi, E. necator and Golovinomyces orontii). The genomes, which were assembled based on various sequencing platforms (PacBio, ABI Solid or Illumina), were surveyed for their repeat content and repeat landscapes for each genome based on % nucleotide divergence to the consensus TE sequences were calculated out of the RepeatMasker output using Perl scripts. Sequence divergence (x-axis) is plotted against frequency (number of sequences; y-axis) for each of the genomes. (PDF 255 kb)
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Frantzeskakis, L., Kracher, B., Kusch, S. et al. Signatures of host specialization and a recent transposable element burst in the dynamic one-speed genome of the fungal barley powdery mildew pathogen. BMC Genomics 19, 381 (2018). https://doi.org/10.1186/s12864-018-4750-6
- Copy number variation
- Evolutionary genomics
- Fungal genomics
- Host specialization
- Transposable elements