ABSTRACT
Long noncoding RNA (lncRNA) plays important roles in sexual development in eukaryotes. In filamentous fungi, however, little is known about the expression and roles of lncRNAs during fruiting body formation. By profiling developmental transcriptomes during the life cycle of the plant-pathogenic fungus Fusarium graminearum, we identified 547 lncRNAs whose expression was highly dynamic, with about 40% peaking at the meiotic stage. Many lncRNAs were found to be antisense to mRNAs, forming 300 sense-antisense pairs. Although small RNAs were produced from these overlapping loci, antisense lncRNAs appeared not to be involved in gene silencing pathways. Genome-wide analysis of small RNA clusters identified many silenced loci at the meiotic stage. However, we found transcriptionally active small RNA clusters, many of which were associated with lncRNAs. Also, we observed that many antisense lncRNAs and their respective sense transcripts were induced in parallel as the fruiting bodies matured. The nonsense-mediated decay (NMD) pathway is known to determine the fates of lncRNAs as well as mRNAs. Thus, we analyzed mutants defective in NMD and identified a subset of lncRNAs that were induced during sexual development but suppressed by NMD during vegetative growth. These results highlight the developmental stage-specific nature and functional potential of lncRNA expression in shaping the fungal fruiting bodies and provide fundamental resources for studying sexual stage-induced lncRNAs.
KEYWORDS: Fusarium graminearum, Xrn1 exonuclease, fruiting body, long noncoding RNAs, perithecia, sexual development
IMPORTANCE
Fusarium graminearum is the causal agent of the head blight on our major staple crops, wheat and corn. The fruiting body formation on the host plants is indispensable for the disease cycle and epidemics. Long noncoding RNA (lncRNA) molecules are emerging as key regulatory components for sexual development in animals and plants. To date, however, there is a paucity of information on the roles of lncRNAs in fungal fruiting body formation. Here we characterized hundreds of lncRNAs that exhibited developmental stage-specific expression patterns during fruiting body formation. Also, we discovered that many lncRNAs were induced in parallel with their overlapping transcripts on the opposite DNA strand during sexual development. Finally, we found a subset of lncRNAs that were regulated by an RNA surveillance system during vegetative growth. This research provides fundamental genomic resources that will spur further investigations on lncRNAs that may play important roles in shaping fungal fruiting bodies.
INTRODUCTION
Genomes of eukaryotes—from simple yeast to animals—are pervasively transcribed from noncoding intergenic regions and in antisense orientation from genic regions (1, 2). Long noncoding RNAs (lncRNAs) are loosely defined as noncoding transcripts longer than 200 nucleotides, which are mostly transcribed by RNA polymerase II and share common features with mRNAs other than protein-coding capacity (3). lncRNAs are versatile molecules that not only regulate gene expression, but also affect enzymatic activities and chromosome conformation (4, 5). Since the discovery of the XIST lncRNA required for X chromosome inactivation (6), the roles of lncRNAs in developmental processes such as embryogenesis and tissue differentiation have been extensively studied in animals along with the advent of transcriptome sequencing (RNA-seq) technologies (7, 8). Yet the full scope of the developmental roles of lncRNAs is far from understood.
In the highly divergent yeasts Saccharomyces cerevisiae (budding yeast) and Schizosaccharomyces pombe (fission yeast), the onset of sexual sporulation and the following meiotic divisions are tightly regulated by elaborate mechanisms involving lncRNAs (9). In budding yeast, a promoter-derived lncRNA suppresses the expression of IME1 (inducer of meiosis 1), the master regulator for the sexual sporulation, by inducing heterochromatin formation in the promoter region of IME1 during vegetative growth (10). In addition, the transcription of another lncRNA antisense to IME4 gene inhibits the expression of IME4 by antagonizing sense transcription (11, 12). Although there is no such conserved or analogous regulatory mechanism in fission yeast, lncRNAs also play diverse roles in sexual sporulation: for example, sequestering RNA elimination factors that repress meiotic gene expression (13–15) and contributing to homologous chromosome pairing (16). Despite the growing evidence of the regulatory roles in yeasts, information on lncRNA expression and function during fruiting body formation in filamentous fungi is scarce.
RNA quality control mechanisms are crucial for the regulation of lncRNA expression in budding yeast. The nuclear exosome is engaged in RNA processing and degradation of transcripts, including lncRNAs that are specifically expressed during sexual sporulation; the deletion of RRP6 encoding the exosome-associated exonuclease resulted in the accumulation of noncoding transcripts that otherwise remained silenced during vegetative growth (17–19). In human cells, promoter-derived transcripts were also ectopically expressed upon deletion of the exosome components, including the homologous RRP6 gene, suggesting the conserved role of the exosome for lncRNA expression in diverse eukaryotes (20). The nonsense-mediated decay (NMD) pathway is another quality control checkpoint for aberrant transcripts in the cytoplasm and recently emerged as a key player for fine-tuning of both coding and noncoding gene expression (21). A genome-wide survey of human lncRNA sequences showed that most lncRNAs harbor short open reading frames (ORFs) that would lead to activation of the NMD pathway (22). In fact, subsets of lncRNAs found in budding yeast, the model plant Arabidopsis, and animals are subject to degradation through the NMD pathway (23–25).
The cytoplasmic exonuclease Xrn1 is the final enzyme responsible for the degradation of decapped and deadenylated transcripts that have been recognized and processed by NMD components. The deletion of XRN1 in budding yeast also leads to the accumulation of more than a thousand cryptic noncoding transcripts termed “XUTs” (Xrn1-sensitive unstable transcripts), most of which are distinct from the noncoding transcripts that arise by exosome depletion (26). Many XUTs are antisense to annotated genes and seemed to have repressive roles in sense transcription by modulating chromatin status of the promoter regions (26).
It has been argued that organismal complexity is correlated with expression dynamics of noncoding transcripts (5, 27–29). In the kingdom Fungi, multicellular fruiting bodies have independently evolved at least twice in the diverging lineages (30, 31). Given the key regulatory roles of lncRNAs in sexual sporulation and morphological transition in yeasts (32, 33), lncRNAs may have exerted their roles in evolution of multicellularity and sexual development in filamentous fungi. Fusarium graminearum is a plant-pathogenic fungus infecting our staple crops, such as wheat and corn, and thus has been a model for studying the developmental process of perithecia, the sexual fruiting bodies of the fungus, as well as other interesting aspects of biology, including host-pathogen interaction and mycotoxin production (34, 35). The fungus is probably the best organism for investigating the lncRNA catalog in fruiting body-forming fungi, as perithecia develop at sufficient synchronicity in culture media, enabling time-series transcriptome analyses with this microscopic organism (36–38). Also, the genome sequence assembly is complete, featuring a total of 4 chromosomes (39), and the genome has been annotated and curated—although it still lacks lncRNA annotations (40, 41). In addition, plentiful genetic resources have accumulated through large-scale functional studies of perithecium development (38, 42–47).
The goal of the present study was to characterize lncRNAs that are specifically expressed in the fungal fruiting body undergoing sexual development and to investigate their developmental stage-specific expression and regulation. We identified lncRNAs with a pipeline that constructs de novo transcript annotations by combining RNA-seq data from vegetative and sexual developmental stages and then removes those with detectable protein-coding potential or a monotonous expression profile. Hundreds of lncRNAs that exhibit dynamic expression patterns were found, thereby expanding the universe of genomes known to have significant noncoding roles in development—specifically, here, the multicellular development of fungal fruiting bodies.
RESULTS
Transcriptional reprogramming during perithecium formation.
To obtain time course transcriptome data during the sexual development of F. graminearum, we sequenced samples from hyphae, strands of cells that make up vegetative stages of most of the fungi (S0), and from five successive sexual stages (S1 to S5 [Fig. 1A]) that capture key morphological transitions during the development of perithecia (48), defined at the formation of the following: S1, perithecial initials (hyphal curls that give rise to the perithecial tissues); S2, perithecial walls; S3, paraphyses (sterile cells supporting perithecia); S4, asci (saclike structures in which ascospores develop); and S5, ascospores (meiospores). A total of 480 million RNA-seq reads were generated from 18 samples (6 stages × 3 replicates), and there were an average of 25 million mapped reads per sample (see Fig. A in Text S1 in the supplemental material). We validated our sampling scheme by perithecial morphology for 3 biological replicates, using the BLIND program (49), which determined the sequence of the developmental time course data without prior information other than gene expression data (see Fig. B in Text S1).
Differentially expressed (DE) genes between any two successive developmental stages (>4-fold at a 5% false-discovery rate [FDR]) were mostly unique compared to other pairwise stage comparisons (Fig. 1B). Overrepresented Gene Ontology database (GO) terms for the stage-specific DE genes reflected key biological processes during the morphological transitions (see Table A in Text S1). For example, the GO term “lipid metabolism” had the highest representation in the “S0 versus S1” comparison, although it was statistically nonsignificant (Fig. 1C). The accumulated lipids in hyphae and perithecial initials are vital for development of paraphyses and asci (50). Perithecia dramatically increased in size and became more rigid during S2 and S3, which is accompanied by GO terms related to carbohydrate metabolism (Fig. 1C). Finally, when the asci develop from the fertile layer during S3 and S4, meiosis-related genes were significantly enriched for GO terms, including “meiotic cell cycle process” and “ascospore formation” at a 5% FDR (Fig. 1C). It is noteworthy that most of the DE genes were upregulated in the later developmental stages (see Fig. C in Text S1), indicating that gene activation is the most common means of gene regulation during sexual development.
Identification of lncRNA in perithecia.
To discover lncRNAs expressed during perithecial development, we adopted an established protocol for novel transcript identification (51), with some modifications (see Fig. D in Text S1). First, we constructed de novo transcript annotations (28,872 transcripts expressed from 20,459 genomic loci) and identified potentially novel transcripts that were absent in the reference annotations (Table 1). For identification of noncoding transcripts, the coding potential of the novel transcripts was computed by using the CPAT program (52). To maximize both sensitivity and specificity for noncoding transcript detection, the program was trained on the F. graminearum genome data set, and the threshold was set to a CPAT score of 0.540 (see Fig. D in Text S1) (cf. 0.364 for humans and 0.440 for mice [53]). The transcripts with a low coding potential (CPAT score of ≤0.540) were further scanned against the Pfam and Rfam databases to filter out transcripts encoding protein domains and harboring any known structural RNA motifs, respectively (E value of <10−10 [Table 1]). Finally we only retained transcripts that were differentially expressed in at least one developmental stage (5% FDR), yielding a total of 547 lncRNA candidates (Table 1; see Table S1 in the supplemental material).
TABLE 1 .
Transcript class (code)a | No. of transcripts |
||
---|---|---|---|
Novelb | Noncodingc | DEd | |
Splicing variants (J) | 5,185 | 92 | 17 |
Tandem transcripts (P) | 740 | 388 | 100 |
Intergenic transcripts (U) | 2,215 | 1,054 | 167 |
Antisense transcripts (X) | 2,892 | 1,040 | 263 |
Sum | 11,032 | 2,574 | 547 |
Transcript class codes were tagged by the gffcompare program (122).
Among a total of 11 transcript class codes, transcripts tagged with the class codes J, P, U, and X were considered novel transcripts (see Text S1 for details).
Noncoding transcripts were identified by the coding potential assessment tool (CPAT) program (52) and further filtered by Pfam and Rfam database searches.
Differentially expressed (DE) noncoding transcripts of at least one developmental stage were identified as F. graminearum lncRNAs.
The identified lncRNAs were distributed across the 4 chromosomes and were generally shorter, with fewer exons than mRNAs (transcripts with a CPAT score of >0.540) (Fig. 2A to C). Based on the relative position to mRNAs, lncRNAs can be classified as antisense lncRNA (ancRNA) or long intergenic ncRNA (lincRNA). There were 280 ancRNAs that overlapped more than 100 bp of an mRNA on the opposite strand and 237 lincRNAs that were situated between annotated genes (Table S1). The mean A/U content of ancRNA and lincRNA sequences falls between the coding sequences of the mRNAs and the intergenic regions (Fig. 2D). These distinctive genomic features of the lncRNA sequences are commonly observed in other eukaryotes (29, 54–57). However, we identified only 5 lncRNAs that showed similarity to lncRNAs in other eukaryotes (E value of <10−10; see Table B in Text S1), suggesting either the poor status of lncRNA annotations in filamentous fungi or a high degree of sequence divergence in fungal lncRNAs.
Developmental expression of lncRNA.
The sexual stage transcriptome data showed predominance of lncRNAs at the meiotic stage (S4), where the expression of many lncRNAs peaked (234 out of 547 [Fig. 2E]). We compared the degree of differential expression of lncRNAs to that of mRNAs (9,457 transcripts differentially expressed in at least one developmental stage at 5% FDR). The ratio of the maximum expression among six developmental stages to the mean expression over the remaining five stages was calculated for lncRNAs and the differentially expressed mRNAs. By this metric, lncRNA was prone to be more differentially expressed than mRNA (P = 2.2 × 10−16; Komolgorov-Smirnov test statistic, D = 0.39), with the third quartile value of the ratio measuring 2.93 for lncRNA and 1.88 for mRNA (Fig. 2F). Also, we identified seven coexpressed clusters of lncRNAs that showed developmental stage-specific expression patterns, suggesting distinct roles of lncRNAs in different stages of perithecial development (Fig. 3A).
In addition to the sexual stage data set, we obtained transcriptome data during spore germination to investigate the degree of lncRNA expression in vegetative stages. The data set was comprised of four spore germination stages: G0, fresh spore; G1, polar growth; G2, doubling of long axis; and G3, branching of hyphae (see Fig. E in Text S1). Overall expression of the lncRNA gradually increased over the course of perithecial development, peaking at S4, while most of the lncRNA remained unexpressed or had low expression in the germination stages, indicating that most of the lncRNA expression is sexual stage specific (Fig. 3B).
Verification of lncRNA production.
To validate lncRNA expression, we chose eight lncRNAs and performed PCR with 3′ rapid amplification of cDNA ends (RACE-PCR) and Sanger sequencing. All the selected lncRNAs were amplified from total RNA extracts, and their polyadenylation sites were determined (see Fig. F in Text S1). Also, to examine if there is an intraspecific conservation in the lncRNA content and expression, we utilized degradome-seq data from another F. graminearum wild-type (WT) strain sampled at the meiotic stage (47). Degradation of lncRNA transcripts expressed at S4 was evident, which in turn confirmed the consistent lncRNA production in the two strains (Fig. 4; also see Fig. 5B below).
Fungal genomes are known for having shorter intergenic spaces than other eukaryotic genomes. Therefore, fungal lncRNAs could be a transcriptional noise arising from neighboring genes. To test this, we examined global patterns of the expression correlation between lncRNA and neighboring genes, with close examination of some selected examples whose expression was confirmed by 3′ RACE-PCR. The lncRNAs antisense to ORC1, ORC2, and CENP-T each had an upstream gene in close proximity on the same strand (Fig. 4; see Fig. F in Text S1). However, the sexual stage expression between the lncRNAs and their respective upstream genes was not correlated (|r| < 0.50 [see Table C in Text S1]). Positive correlation was observed in expression levels between lncRNAs and their divergently transcribed genes as in the HIR1 and NSE4 loci (r > 0.8 [Fig. 4; see Table C in Text S1]), indicating prevalence of bidirectional promoters for lncRNA transcription (2, 58, 59). On the other hand, the expression of lncRNAs and their convergently transcribed genes tend not to be correlated, as in the CENP-T and RMD1 loci (|r| < 0.50 [Fig. 4; see Table C in Text S1]). These patterns were globally observed in lncRNA-associated loci (see Fig. F in Text S1), suggesting that the lncRNAs were not likely to be misannotated extensions of neighboring genes (54, 60, 61).
Identification of sRNA-enriched loci associated with lncRNAs.
We found 300 sense mRNA-ancRNA pairs with different orientations: 5′→5′ partial, 3′→3′ partial, and full overlaps. One of the most common mechanisms involving antisense transcription is the RNA interference (RNAi) pathway incorporating small RNAs (sRNAs) generated from the double-stranded RNA regions. To investigate the degree and effect of sRNA production in the ancRNA loci, we analyzed the previously published sRNA-seq and degradome-seq data at the meiotic stage (47). As expected, sRNA reads were mapped at a higher frequency to ancRNAs than to mRNAs without overlapping antisense transcripts, the sense mRNAs, or lincRNAs (P < 1.2 × 10−8; Kruskal-Wallis test statistic, H = 155 [Fig. 5A]), suggesting that the ancRNA loci may serve as a major source for endogenous sRNA production. However, the correlation of the degradome-seq and our RNA-seq data at S4 showed that sRNA-mediated endonucleolytic cleavage of ancRNAs and sense mRNAs was comparable to that of mRNAs without antisense transcripts (Fig. 5B), implying that the ancRNA loci were not preferentially targeted by RNAi machinery, posttranscriptionally.
It remains paradoxical that gene silencing induced by heterochromatin formation requires sRNA production via cotranscriptional processes, sometimes from lncRNAs (62–66). To search for any lncRNAs associated with sRNA-enriched loci that could be indicative of transcriptional gene silencing events, we examined the top 80 sRNA clusters ranked by the number of mapped reads, which accounted for 62% of mapped sRNA reads (see Table D in Text S1). Production of sRNAs in the top 80 clusters was dependent on Dicers and Argonautes (47), indicating that the sRNAs were produced by RNAi machinery (Fig. 5C). Most of the sRNA clusters were found in genic regions, containing at least one annotated gene, to which a large portion of sRNA reads were mapped (Fig. 5D). We observed that the coding genes closest to the centers of sRNA clusters exhibited overall low expression (<0.5 read per kilobase per million [RPKM] in 22 out of the 80 clusters) (Fig. 5D). A significant portion of sRNAs were also derived from noncoding transcripts and genic regions overlapped with antisense transcripts, some of which were identified as lncRNAs (Fig. 5D; see Fig. S1 in the supplemental material). Unexpectedly, the lncRNAs associated with sRNA clusters exhibited moderate expression (n = 19; median expression of 5.2 RPKM). In addition, the coding genes closest to the centers of the sRNA clusters showed higher expression levels (n = 19; median expression of 4.0 RPKM) than those without an associated lncRNA (n = 61; median expression of 1.3 RPKM; P = 0.029; Mann-Whitney test statistic, U = 747).
Coexpression of lncRNAs and their sense transcripts.
We could not find strong evidence for sRNA-mediated transcriptional and posttranscriptional gene silencing in the ancRNA loci. Interestingly, we did observe gene expression correlation in many ancRNAs and sense mRNA pairs across the sexual stages (85 out of the 300 pairs with Pearson’s correlation |r| > 0.70; Fisher’s exact test, P < 0.05 [Fig. 6]), most of which were positively correlated (76 out of the 85 pairs). We asked whether the ancRNAs are antisense to genes involved in a specific biological process. We found that 17 genes in the ancRNA loci were involved in DNA metabolic processes such as DNA replication, repair, and recombination (Table 2). Notably, the positively correlated sense mRNAs were enriched for the GO term “DNA metabolism” at a 5% FDR (8 out of the 76 genes [see Table E in Text S1]), and among them, five genes (FGRRES_00736, FGRRES_01614, FGRRES_06286, FGRRES_07280, and FGRRES_08658) appeared to have functions related to DNA damage repair (Table 2). In addition, we surveyed previously published research for the 295 sense genes to determine if there are any genes known to affect sexual development. We found one gene, RGSC (FGRRES_09585; encoding a regulator of G proteins), whose knockout phenotype was defective in ascospore morphology (67).
TABLE 2 .
Gene ID no. | Putative function | Protein domain (E value)a | Correlation with ancRNAb |
---|---|---|---|
FGRRES_00667 | Similar to chromatin assembly complex subunit p60 | Pfam12894 (3.69e−08) | 0.76 (lncRNA-026) |
FGRRES_00736 | Similar to DNA damage response protein WSS1 | Pfam08325 (3.75e−79) | 0.89 (lncRNA-030) |
FGRRES_01336 | Origin recognition complex subunit 1 | Cd04720 (3.48e−37) | 0.69 (lncRNA-065) |
FGRRES_01614 | Similar to DNA mismatch repair protein MLH3 | COG0323 (5.15e−39) | 0.88 (lncRNA-083) |
FGRRES_05344 | Histone regulatory protein 1 (HIR1) | Pfam07569 (6.27e−99) | 0.29 (lncRNA-324) |
FGRRES_05737 | ssDNA/RNA-binding protein | Pfam00076 (1.73e−15) | 0.91 (lncRNA-342) |
FGRRES_05781 | Similar to TCB2 transposase | Pfam01498 (3.32e−08) | 0.97 (lncRNA-344) |
FGRRES_06122 | Origin recognition complex subunit 2 | Pfam04084 (3.98e−163) | 0.39 (lncRNA-356) |
FGRRES_06231 | Origin recognition complex subunit 4 | Pfam14629 (1.82e−70) | 0.01 (lncRNA-367) |
FGRRES_06286 | Similar to DNA repair polymerase RAD30 | Cd01703 (6.27e−145) | 0.75 (lncRNA-369) |
FGRRES_06339 | DNA primase small subunit | Pfam01896 (8.59e−42) | 0.40 (lncRNA-373) |
FGRRES_07280 | Similar to DNA repair helicase ERCC3/RAD25 | Pfam16203 (6.04e−173) | 0.70 (lncRNA-461) |
FGRRES_08650 | Similar to SEN1 helicase | Pfam12726 (0e+00) | 0.66 (lncRNA-214) |
FGRRES_08658 | Similar to DNA repair endonuclease ERCC4/RAD16 | Pfam02732 (2.80e−25) | 0.77 (lncRNA-216) |
FGRRES_09872 | Similar to DNA repair dioxygenase AlkB | COG3145 (4.37e−07) | −0.02 (lncRNA-144) |
FGRRES_16954 | Centromere protein T (CENP-T) | Pfam15511 (6.41e−47) | −0.36 (lncRNA-235) |
FGRRES_17018 | Nonstructural maintenance of chromosome element 4 (NSE4) | Pfam08743 (3.83e−45) | 0.10 (lncRNA-201) |
BLAST search for associated protein domains related to DNA metabolic processes.
Pearson’s correlation for the expression levels of sense transcripts and ancRNAs across the sexual development stages. Values greater than 0.7 are marked in boldface.
Identification of lncRNAs affected by the NMD pathway.
The NMD pathway is known to regulate the expression of noncoding genes, as well as coding genes, for sexual sporulation in yeasts. To identify the sexual stage-induced lncRNAs that were affected by NMD, we generated a deletion strain lacking XRN1 (FGRRES_06799) that encodes a 5′→3′ exonuclease. The Δxrn1 deletion mutant displayed a lower growth rate on different growth media compared to the wild type (WT); however, it produced normal-shaped asexual spores (Fig. 7A; see Fig. G in Text S1). We observed that perithecial development was significantly delayed and ascus development was defective in the Δxrn1 strain, producing variable ascospore sizes (Fig. 7A; see Fig. G in Text S1). The defective sexual phenotype was restored by genetic complementation with XRN1 (see Fig. G in Text S1).
To identify lncRNA whose expression was affected by NMD activity, we analyzed the transcriptome data from the WT and the Δxrn1 strain at the vegetative (S0) and meiotic (S4) stages. The transcriptome data of the Δxrn1 strain were distinct from, but most similar to, those of WT at the corresponding stages, indicating drastic effects of XRN1 on gene expression levels as a major component for RNA turnover (Fig. 7B). After expression values were normalized with 124 ribosomal protein genes that were known to be relatively insensitive to NMD activity (26), we identified a total of 1,122 XUTs that were differentially expressed at S0 or S4 in the Δxrn1 strain (>3-fold increase at 5% FDR [Fig. 7C; see Table S2 in the supplemental material]). After the normalization, the XUTs identified at S0 and S4 showed median 5.0- and 5.8-fold increases in the Δxrn1 mutant, respectively (Fig. 7D; Table S2). Many XUTs were previously annotated transcripts or isoforms of them (70% [781/1,122]), and only 11% of XUTs (122/1,122) were predicted to be noncoding transcripts (CPAT score of ≤0.540) (Table S2). Among the noncoding XUTs, we identified 25 lncRNAs whose expression was elevated upon the Xrn1 depletion at S0 and showed increasing patterns across the sexual stages (Fig. 7E; see Fig. S2 in the supplemental material). In addition, many of the coding XUTs identified at S0 were also induced as the sexual development progressed (see Fig. H in Text S1). Interestingly, we found that key components of the RNA-induced silencing complex (RISC) (68) were also identified as XUTs, such as DICER2 (FGRRES_04408), AGO1 (FGRRES_16976), Neurospora crassa QIP homologue (FGRRES_06722), and RDRP genes (coding for RNA-dependent RNA polymerases [FGRRES_01582, _04619, and _09076]).
DISCUSSION
Here we profiled transcriptomes of vegetative and sexual stages that span the entire life cycle of F. graminearum. lncRNAs are usually an order of magnitude less abundant than mRNAs (69, 70), so the unprecedented depth of the sequencing data we generated (total of 938 million mapped reads) enabled us to capture scantly expressed noncoding transcripts. This study has revealed global properties of lncRNAs during perithecial development, characterized by dynamic and developmental stage-specific expression. In the last step of our lncRNA identification pipeline, we only included differentially expressed noncoding transcripts to discern lncRNAs of biological significance. This filtering step allowed us to identify low-abundance lncRNAs that alone could be argued to be transcriptional noise (71, 72). For many antisense lncRNAs, we detected parallel induction with their respective sense transcripts across sexual development and identified a subset of lncRNAs that are sensitive to NMD activity before sexual induction.
Our lists of F. graminearum lncRNAs contain many confident lncRNA annotations, but are still far from complete. This is primarily due to difficulty in unequivocal determination of whether a transcript is coding or noncoding (73). Although protein products from most of the bona fide lncRNAs with predicted ORFs have not been detected in cells (74, 75), many lncRNAs with one or more ORFs have been shown to be associated with ribosomes in budding yeast, Arabidopsis, and animals (76–81). By scrutinizing the sRNA-enriched loci, we identified several transcripts with short ORFs (ranging from 49 to 227 amino acids) as putative lncRNAs. These novel transcripts were initially filtered out by the CPAT program; however, another annotation tool, CPC2 (82), classified them as lncRNAs, and the lncRNA annotations were also supported by the lack of cross-species conservation of the deduced polypeptides (E value of ≥10−10 [see Table F in Text S1]).
Another source of false negatives in our data set may have arisen from poly(A)-based library preparation that excluded some lncRNAs lacking poly(A) tail. This may account for the inclusion of fewer lncRNAs in our XUT identification process, as deadenylation often takes place prior to 5′→3′ degradation by Xrn1. More precise identification of lncRNAs, especially for those undergoing deadenylation by the RNA quality control machineries, should be accompanied by cap analysis gene expression (CAGE)-seq (83–85). However, most lncRNAs identified in this study were also detected by degradome-seq (47), another sequencing method (also known as parallel analysis of RNA ends [86]), which further validates their authenticity.
To better understand how the expression of lncRNAs was controlled during perithecial development, we identified XUTs, as the NMD pathway has been shown to determine the fate of lncRNAs (21, 84). However, only 5% of the sexual stage-induced lncRNAs (25/547) were affected by Xrn1 activity, and the majority of the lncRNAs seemed to escape from the RNA surveillance system. The proportion of XUTs among the lncRNAs in F. graminearum is comparable to that in other eukaryotes, where approximately 4 to 14% of noncoding transcripts are known to undergo NMD (25). Interestingly, sexually induced RISC components were highly upregulated in the Δxrn1 mutant, indicating a possible link between the gene silencing pathway and the NMD pathway. Further studies on lncRNAs and the RNAi machinery that were affected by NMD activity will provide novel insights into regulatory mechanisms via altered RNA metabolism during sexual development.
We initially aimed to dissect the roles of other exosome and NMD components in lncRNA expression, such as RRP6 (FGRRES_06049), DBP2 (FGRRES_16145), and MTR4 (FGRRES_01656) (84, 87). However, efforts to obtain deletion strains lacking either the DBP2, MTR4, or RRP6 gene were unsuccessful (W. Kim and F. Trail, unpublished data), suggesting these genes may be essential in F. graminearum, as they are in another filamentous fungus, Neurospora crassa (88, 89). In fission yeast, the nuclear exosome mediates gene silencing of coding and noncoding loci during vegetative growth, and the sexual sporulation is triggered by disassembly of heterochromatin on the silenced loci (90). Therefore, it will be interesting to see if the regulation of lncRNA expression is achieved by modulation of chromatin status before and after the sexual induction in F. graminearum.
Antisense transcription can influence synthesis, expression kinetics, and stability of sense transcripts through a variety of mechanisms (5, 91). Antagonism of lncRNAs against meiotic gene expression has been documented in yeasts (10, 11, 92–95). Nevertheless, there has been growing evidence that lncRNAs activate repressed genes by modulating local chromatin structures, which can facilitate coordinated gene expression in budding yeast (96, 97) and other eukaryotes (98–101). In favor of this regulatory phenomenon, we hypothesize that the F. graminearum lncRNAs, which showed parallel induction with DNA metabolism-related genes across the sexual development stages, may play a role during meiosis that requires DNA break and repair for homologous recombination, according to “guilt by association” (1, 29). However, lncRNAs often exhibited cell-type-specific expression (100, 102, 103) and even allele-specific expression within the same nucleus (104). Therefore, we cannot rule out the possibility that the positively correlated pairs of lncRNA and sense transcript are in fact mutually exclusively expressed in different tissues or cell types in the perithecia, inhibiting each other.
Although genes found in sRNA-enriched loci are usually silenced by RNAi-dependent heterochromatin formation, some of the sRNA clusters involving lncRNAs, paradoxically, were transcriptionally active at the meiotic stage in F. graminearum. In our developmental transcriptome data, we observed that many stage-specific genes were induced over the course of sexual development, which may play key roles in the corresponding perithecial tissue development. It is conceivable that the silenced genes in vegetative tissues were derepressed by lncRNA expression by yet unknown mechanisms upon sexual induction. In N. crassa, molecular studies on the circadian clock gene locus revealed a periodic gene activation and repression mechanism involving lncRNA and facultative heterochromatin formation. The expression of an lncRNA antisense to the circadian clock gene promotes sense transcription by generating a more transcriptionally permissive chromatin that has been silenced by sRNA-mediated heterochromatin formation (105).
This study presents genome-wide characterization of lncRNAs during fruiting body development. The transcriptome landscape, including lncRNAs during the life cycle of F. graminearum, provides fundamental genomic resources to the Fusarium community. The detailed molecular study of newly identified lncRNAs, with its established tools for rapid genetic analyses and ample genetic resources, will contribute to the understanding of how fungi utilize noncoding genomes for laying out their multicellular body plan.
MATERIALS AND METHODS
Data generation and processing.
The F. graminearum genome assembly (39) and the Ensembl annotation version 32 (40) of wild-type strain PH-1 (accession no. FGSC 9075 and NRRL 31084) were used throughout this study. For total RNA extraction, synchronized fungal tissues were collected from carrot agar cultures at the previously defined developmental stages during perithecial formation (36–38, 48). For transcriptome data of spore germination stages, asexual spores (macroconidia) were spread on Bird agar medium (106) overlaid with a cellophane membrane and sampled at the indicated spore germination stages (see Fig. E in Text S1). Strand-specific cDNA libraries were constructed from poly(A)-captured RNAs, using the Kapa stranded RNA-Seq library preparation kit (Kapa Biosystems, Wilmington, MA), and sequenced on the Illumina HiSeq 2500 platform (Illumina, Inc., San Diego, CA) at the Michigan State University Research Technology Support Facility (https://rtsf.natsci.msu.edu/genomics). Following quality control for raw reads (Text S1), filtered reads were mapped to the repeat-masked genome using the HISAT2 program (v2.0.4) (107), and a genome-guided transcriptome assembly was performed using the StringTie program (v1.3.0) to generate de novo transcript annotations (108).
Differential expression and functional enrichment analyses.
Read counts for gene loci were calculated using the htseq-count program (v0.6.1) (109). On average, 87% of mapped reads were overlapped to exons in the de novo annotations. Gene expression levels in counts per million (CPM) values were computed and normalized by effective library size estimated by trimmed mean of M values, using the edgeR R package (v3.14.0) (110). Only genes with CPM values greater than 1 in at least 3 samples were kept for further analyses (15,476 out of 20,459 gene loci). Then, differentially expressed (DE) genes showing greater than 4-fold difference at an FDR of 5% were identified between two successive developmental stages, using the limma R package (v3.28.21) (111). GO terms were assigned to the de novo annotations, using the Trinotate program (v3.0.1) (112). The list of GO terms was customized by adding several GO terms related to developmental processes to the GO Slim terms specific for fission yeast (113). Functional enrichment analyses for DE genes were performed using the GOseq R package (v1.24.0), including only those genes annotated by one or more GO terms (114). To assess enrichment of GO terms, the Wallenius approximation (an extension of the hypergeometric distribution) and Benjamini-Hochberg method were used to calculate the FDR-corrected P value.
Conserved lncRNA search.
To search for conserved lncRNAs, the 547 lncRNAs were queried against the RNAcentral database version 5 (http://rnacentral.org), using the nhmmer program, which detects remote homologies, in the HMMER software (v3.1b2) (115). Search hits with an E value of <10−10 were reported.
Coexpression network analysis.
The weighted gene correlation network analysis (WGCNA) R package (v1.51) (116) was used to cluster lncRNAs by averaged RPKM values for developmental stages. The “pickSoftThreshold” function was used to determine soft-thresholding power that measures the strength of correlation based on not just the direct correlation value of pairs of genes, but also the weighted correlations of all of their shared neighbors in the network space (117). The soft-thresholding power of 26 was selected, which is the lowest power for which the scale-free topology model fit index reaches 0.80. A range of treecut values were tested for cluster detection, and the value was set to 0.18 (corresponding to a correlation of 0.82). All other WGCNA parameters remained at their default settings.
Identification of small RNA clusters.
The sRNA-seq and degradome-seq data were obtained from NCBI GEO (GSE87835) and NCBI SRA (PRJNA348145), respectively (47). In filamentous fungi, the size of a majority of sRNAs ranges from 17 to 27 nucleotides (nt), with a strong 5′ U preference (70 to 82%) (47, 118). Thus, clusters of 17- to 27-nt-long 5′-U sRNA reads were detected across the genome, using the ShortStack program (v3.8.2) (119) with the option arguments “--pad 22” and “--mincov 20.” Subsequently, the number of 5′ U sRNA reads aligned to different genomic features (e.g., coding regions) were counted for each sRNA cluster, using the htseq-count program (v0.8.0) (109). The degradome-seq data set was processed according to the previous study (47).
Expression correlation analysis.
The expression value matrix for the 18 RNA-seq data (6 stages × 3 replicates) were rearranged by the BLIND program (see Fig. B in Text S1). Pearson’s correlation and the associated P value by Fisher’s exact test were calculated for the expression levels of the 300 sense mRNA-antisense lncRNA pairs, using an R script (29). For sense mRNAs only, which showed positive correlation with antisense lncRNAs, we performed functional enrichment analyses, using the GOseq R package (v1.24.0) (114), as done for DE genes between two successive developmental stages (see above).
XUT identification.
Generation, confirmation, and complementation of the Δxrn1 mutant are described in Text S1, and the primers used in this study are listed in Table S3 in the supplemental material. To incorporate novel transcripts that were only expressed in the Δxrn1 mutant due to loss of NMD activity, the RNA-seq reads for the Δxrn1 mutant were independently processed, and the assembled transcripts were merged to the de novo annotations, using the “merge” function in the StringTie program (v1.3.0) (108). Transcript abundance is globally affected by XRN1 deletion in budding yeast; however, the expression of ribosomal protein genes shows only slight increases in the Δxrn1 mutant and remains constant after lithium treatment, which inhibits 5′→3′ exonuclease activities (26, 120). Thus, before XUT identification, expression values were normalized in such a way that ribosomal protein genes are expressed at the same levels in the WT and Δxrn1 mutant by multiplying by 0.66 and 1.96 the RPKM values of the WT at S0 and S4, respectively (see Fig. I in Text S1). Differential expression analyses were performed, using the “stattest” function with the option argument “libadjust = FALSE” in the Ballgown R package (v2.8.4) (121). The DE transcripts showing a 3-fold increase in the Δxrn1 mutant were identified as XUTs (5% FDR). We excluded transcripts with relatively low expression levels in the Δxrn1 mutant (<3.0 RPKM) from the putative XUTs to reduce possible false positives.
Accession number(s).
The RNA-seq data generated in the present work have been deposited in NCBI’s Gene Expression Omnibus (https://www.ncbi.nlm.nih.gov/geo) and are accessible through GEO series accession no. GSE109095, which is composed of the two data sets—the sexual stage and Δxrn1 mutant data set (GSE109094) and the spore germination stage data set (GSE109088).
ACKNOWLEDGMENTS
We thank Brad Cavinder, Kevin Childs, and Nicholas Panchy (Michigan State University, East Lansing, MI) for helpful discussion on analyzing data and for providing Perl and Python scripts.
This publication is based upon work supported by the National Science Foundation under grant no. 1456482 to F.T. and Michigan AgBioResearch (to F.T.). Also, this work was supported by Program Area: Plant Health and Production and Plant Products under grant no. 2015-67013-22932 to F.T. from the USDA National Institute of Food and Agriculture. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Any opinions, findings, conclusions, or recommendations expressed in this publication are those of the authors and do not necessarily reflect the view of the U.S. Department of Agriculture and the National Science Foundation.
Footnotes
Citation Kim W, Miguel-Rojas C, Wang J, Townsend JP, Trail F. 2018. Developmental dynamics of long noncoding RNA expression during sexual fruiting body formation in Fusarium graminearum. mBio 9:e01292-18. https://doi.org/10.1128/mBio.01292-18.
REFERENCES
- 1.Guttman M, Amit I, Garber M, French C, Lin MF, Feldser D, Huarte M, Zuk O, Carey BW, Cassady JP, Cabili MN, Jaenisch R, Mikkelsen TS, Jacks T, Hacohen N, Bernstein BE, Kellis M, Regev A, Rinn JL, Lander ES. 2009. Chromatin signature reveals over a thousand highly conserved large non-coding RNAs in mammals. Nature 458:223–227. doi: 10.1038/nature07672. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 2.Xu Z, Wei W, Gagneur J, Perocchi F, Clauder-Münster S, Camblong J, Guffanti E, Stutz F, Huber W, Steinmetz LM. 2009. Bidirectional promoters generate pervasive transcription in yeast. Nature 457:1033–1037. doi: 10.1038/nature07728. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 3.Kapranov P, Cheng J, Dike S, Nix DA, Duttagupta R, Willingham AT, Stadler PF, Hertel J, Hackermüller J, Hofacker IL, Bell I, Cheung E, Drenkow J, Dumais E, Patel S, Helt G, Ganesh M, Ghosh S, Piccolboni A, Sementchenko V, Tammana H, Gingeras TR. 2007. RNA maps reveal new RNA classes and a possible function for pervasive transcription. Science 316:1484–1488. doi: 10.1126/science.1138341. [DOI] [PubMed] [Google Scholar]
- 4.Rinn JL, Chang HY. 2012. Genome regulation by long noncoding RNAs. Annu Rev Biochem 81:145–166. doi: 10.1146/annurev-biochem-051410-092902. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 5.Quinn JJ, Chang HY. 2016. Unique features of long non-coding RNA biogenesis and function. Nat Rev Genet 17:47–62. doi: 10.1038/nrg.2015.10. [DOI] [PubMed] [Google Scholar]
- 6.Brockdorff N, Ashworth A, Kay GF, McCabe VM, Norris DP, Cooper PJ, Swift S, Rastan S. 1992. The product of the mouse Xist gene is a 15 kb inactive X-specific transcript containing no conserved ORF and located in the nucleus. Cell 71:515–526. doi: 10.1016/0092-8674(92)90519-I. [DOI] [PubMed] [Google Scholar]
- 7.Fatica A, Bozzoni I. 2014. Long non-coding RNAs: new players in cell differentiation and development. Nat Rev Genet 15:7–21. doi: 10.1038/nrg3606. [DOI] [PubMed] [Google Scholar]
- 8.Flynn RA, Chang HY. 2014. Long noncoding RNAs in cell fate programming and reprogramming. Cell Stem Cell 14:752–761. doi: 10.1016/j.stem.2014.05.014. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 9.Hiriart E, Verdel A. 2013. Long noncoding RNA-based chromatin control of germ cell differentiation: a yeast perspective. Chromosome Res 21:653–663. doi: 10.1007/s10577-013-9393-5. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 10.van Werven FJ, Neuert G, Hendrick N, Lardenois A, Buratowski S, van Oudenaarden A, Primig M, Amon A. 2012. Transcription of two long non-coding RNAs mediates mating type control of gametogenesis in budding yeast. Cell 150:1170–1181. doi: 10.1016/j.cell.2012.06.049. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 11.Hongay CF, Grisafi PL, Galitski T, Fink GR. 2006. Antisense transcription controls cell fate in Saccharomyces cerevisiae. Cell 127:735–745. doi: 10.1016/j.cell.2006.09.038. [DOI] [PubMed] [Google Scholar]
- 12.Gelfand B, Mead J, Bruning A, Apostolopoulos N, Tadigotla V, Nagaraj V, Sengupta AM, Vershon AK. 2011. Regulated antisense transcription controls expression of cell-type-specific genes in yeast. Mol Cell Biol 31:1701–1709. doi: 10.1128/MCB.01071-10. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 13.Harigaya Y, Tanaka H, Yamanaka S, Tanaka K, Watanabe Y, Tsutsumi C, Chikashige Y, Hiraoka Y, Yamashita A, Yamamoto M. 2006. Selective elimination of messenger RNA prevents an incidence of untimely meiosis. Nature 442:45–50. doi: 10.1038/nature04881. [DOI] [PubMed] [Google Scholar]
- 14.Hiriart E, Vavasseur A, Touat-Todeschini L, Yamashita A, Gilquin B, Lambert E, Perot J, Shichino Y, Nazaret N, Boyault C, Lachuer J, Perazza D, Yamamoto M, Verdel A. 2012. Mmi1 RNA surveillance machinery directs RNAi complex RITS to specific meiotic genes in fission yeast. EMBO J 31:2296–2308. doi: 10.1038/emboj.2012.105. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 15.Yamashita A, Shichino Y, Tanaka H, Hiriart E, Touat-Todeschini L, Vavasseur A, Ding DQ, Hiraoka Y, Verdel A, Yamamoto M. 2012. Hexanucleotide motifs mediate recruitment of the RNA elimination machinery to silent meiotic genes. Open Biol 2:120014. doi: 10.1098/rsob.120014. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 16.Ding DQ, Okamasa K, Yamane M, Tsutsumi C, Haraguchi T, Yamamoto M, Hiraoka Y. 2012. Meiosis-specific noncoding RNA mediates robust pairing of homologous chromosomes in meiosis. Science 336:732–736. doi: 10.1126/science.1219518. [DOI] [PubMed] [Google Scholar]
- 17.Davis CA, Ares M. 2006. Accumulation of unstable promoter-associated transcripts upon loss of the nuclear exosome subunit Rrp6p in Saccharomyces cerevisiae. Proc Natl Acad Sci U S A 103:3262–3267. doi: 10.1073/pnas.0507783103. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 18.Camblong J, Iglesias N, Fickentscher C, Dieppois G, Stutz F. 2007. Antisense RNA stabilization induces transcriptional gene silencing via histone deacetylation in S. cerevisiae. Cell 131:706–717. doi: 10.1016/j.cell.2007.09.014. [DOI] [PubMed] [Google Scholar]
- 19.Lardenois A, Liu Y, Walther T, Chalmel F, Evrard B, Granovskaia M, Chu A, Davis RW, Steinmetz LM, Primig M. 2011. Execution of the meiotic noncoding RNA expression program and the onset of gametogenesis in yeast require the conserved exosome subunit Rrp6. Proc Natl Acad Sci U S A 108:1058–1063. doi: 10.1073/pnas.1016459108. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 20.Preker P, Nielsen J, Kammler S, Lykke-Andersen S, Christensen MS, Mapendano CK, Schierup MH, Jensen TH. 2008. RNA exosome depletion reveals transcription upstream of active human promoters. Science 322:1851–1854. doi: 10.1126/science.1164096. [DOI] [PubMed] [Google Scholar]
- 21.Smith JE, Baker KE. 2015. Nonsense-mediated RNA decay—a switch and dial for regulating gene expression. BioEssays 37:612–623. doi: 10.1002/bies.201500007. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 22.Niazi F, Valadkhan S. 2012. Computational analysis of functional long noncoding RNAs reveals lack of peptide-coding capacity and parallels with 3′ UTRs. RNA 18:825–843. doi: 10.1261/rna.029520.111. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 23.Kurihara Y, Matsui A, Hanada K, Kawashima M, Ishida J, Morosawa T, Tanaka M, Kaminuma E, Mochizuki Y, Matsushima A, Toyoda T, Shinozaki K, Seki M. 2009. Genome-wide suppression of aberrant mRNA-like noncoding RNAs by NMD in Arabidopsis. Proc Natl Acad Sci U S A 106:2453–2458. doi: 10.1073/pnas.0808902106. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 24.Tani H, Torimura M, Akimitsu N. 2013. The RNA degradation pathway regulates the function of GAS5 a non-coding RNA in mammalian cells. PLoS One 8:e55684. doi: 10.1371/journal.pone.0055684. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 25.Ruiz-Orera J, Messeguer X, Subirana JA, Alba MM. 2014. Long non-coding RNAs as a source of new peptides. eLife 3:e03523. doi: 10.7554/eLife.03523. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 26.van Dijk EL, Chen CL, d’Aubenton-Carafa Y, Gourvennec S, Kwapisz M, Roche V, Bertrand C, Silvain M, Legoix-Né P, Loeillet S, Nicolas A, Thermes C, Morillon A. 2011. XUTs are a class of Xrn1-sensitive antisense regulatory non-coding RNA in yeast. Nature 475:114–117. doi: 10.1038/nature10118. [DOI] [PubMed] [Google Scholar]
- 27.Mattick JS, Taft RJ, Faulkner GJ. 2010. A global view of genomic information—moving beyond the gene and the master regulator. Trends Genet 26:21–28. doi: 10.1016/j.tig.2009.11.002. [DOI] [PubMed] [Google Scholar]
- 28.Liu G, Mattick JS, Taft RJ. 2013. A meta-analysis of the genomic and transcriptomic composition of complex life. Cell Cycle 12:2061–2072. doi: 10.4161/cc.25134. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 29.Gaiti F, Fernandez-Valverde SL, Nakanishi N, Calcino AD, Yanai I, Tanurdzic M, Degnan BM. 2015. Dynamic and widespread lncRNA expression in a sponge and the origin of animal complexity. Mol Biol Evol 32:2367–2382. doi: 10.1093/molbev/msv117. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 30.Knoll AH. 2011. The multiple origins of complex multicellularity. Annu Rev Earth Planet Sci 39:217–239. doi: 10.1146/annurev.earth.031208.100209. [DOI] [Google Scholar]
- 31.Nguyen TA, Cissé OH, Yun Wong JY, Zheng P, Hewitt D, Nowrousian M, Stajich JE, Jedd G. 2017. Innovation and constraint leading to complex multicellularity in the Ascomycota. Nat Commun 8:14444. doi: 10.1038/ncomms14444. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 32.Bumgarner SL, Dowell RD, Grisafi P, Gifford DK, Fink GR. 2009. Toggle involving cis-interfering noncoding RNAs controls variegated gene expression in yeast. Proc Natl Acad Sci U S A 106:18321–18326. doi: 10.1073/pnas.0909641106. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 33.Chacko N, Zhao Y, Yang E, Wang L, Cai JJ, Lin X. 2015. The lncRNA RZE1 controls cryptococcal morphological transition. PLoS Genet 11:e1005692. doi: 10.1371/journal.pgen.1005692. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 34.Trail F. 2009. For blighted waves of grain: Fusarium graminearum in the postgenomics era. Plant Physiol 149:103–110. doi: 10.1104/pp.108.129684. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 35.Ma LJ, Geiser DM, Proctor RH, Rooney AP, O’Donnell K, Trail F, Gardiner DM, Manners JM, Kazan K. 2013. Fusarium pathogenomics. Annu Rev Microbiol 67:399–416. doi: 10.1146/annurev-micro-092412-155650. [DOI] [PubMed] [Google Scholar]
- 36.Hallen HE, Huebner M, Shiu SH, Güldener U, Trail F. 2007. Gene expression shifts during perithecium development in Gibberella zeae (anamorph Fusarium graminearum), with particular emphasis on ion transport proteins. Fungal Genet Biol 44:1146–1156. doi: 10.1016/j.fgb.2007.04.007. [DOI] [PubMed] [Google Scholar]
- 37.Sikhakolli UR, López-Giráldez F, Li N, Common R, Townsend JP, Trail F. 2012. Transcriptome analyses during fruiting body formation in Fusarium graminearum and Fusarium verticillioides reflect species life history and ecology. Fungal Genet Biol 49:663–673. doi: 10.1016/j.fgb.2012.05.009. [DOI] [PubMed] [Google Scholar]
- 38.Trail F, Wang Z, Stefanko K, Cubba C, Townsend JP. 2017. The ancestral levels of transcription and the evolution of sexual phenotypes in filamentous fungi. PLoS Genet 13:e1006867. doi: 10.1371/journal.pgen.1006867. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 39.Cuomo CA, Güldener U, Xu JR, Trail F, Turgeon BG, Di Pietro A, Walton JD, Ma LJ, Baker SE, Rep M, Adam G, Antoniw J, Baldwin T, Calvo S, Chang YL, DeCaprio D, Gale LR, Gnerre S, Goswami RS, Hammond-Kosack K, Harris LJ, Hilburn K, Kennell JC, Kroken S, Magnuson JK, Mannhaupt G, Mauceli E, Mewes HW, Mitterbauer R, Muehlbauer G, Münsterkötter M, Nelson D, O’Donnell K, Ouellet T, Qi W, Quesneville H, Roncero MIG, Seong KY, Tetko IV, Urban M, Waalwijk C, Ward TJ, Yao J, Birren BW, Kistler HC. 2007. The Fusarium graminearum genome reveals a link between localized polymorphism and pathogen specialization. Science 317:1400–1402. doi: 10.1126/science.1143708. [DOI] [PubMed] [Google Scholar]
- 40.King R, Urban M, Hammond-Kosack MCU, Hassani-Pak K, Hammond-Kosack KE. 2015. The completed genome sequence of the pathogenic ascomycete fungus Fusarium graminearum. BMC Genomics 16:544. doi: 10.1186/s12864-015-1756-1. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 41.King R, Urban M, Hammond-Kosack KE. 2017. Annotation of Fusarium graminearum (PH-1) version 5.0. Genome Announc 5:e01479-16. doi: 10.1128/genomeA.01479-16. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 42.Son H, Seo YS, Min K, Park AR, Lee J, Jin JM, Lin Y, Cao P, Hong SY, Kim EK, Lee SH, Cho A, Lee S, Kim MG, Kim Y, Kim JE, Kim JC, Choi GJ, Yun SH, Lim JY, Kim M, Lee YH, Choi YD, Lee YW. 2011. A phenome-based functional analysis of transcription factors in the cereal head blight fungus, Fusarium graminearum. PLoS Pathog 7:e1002310. doi: 10.1371/journal.ppat.1002310. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 43.Wang C, Zhang S, Hou R, Zhao Z, Zheng Q, Xu Q, Zheng D, Wang G, Liu H, Gao X, Ma JW, Kistler HC, Kang Z, Xu JR. 2011. Functional analysis of the kinome of the wheat scab fungus Fusarium graminearum. PLoS Pathog 7:e1002460. doi: 10.1371/journal.ppat.1002460. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 44.Yun Y, Liu Z, Yin Y, Jiang J, Chen Y, Xu JR, Ma Z. 2015. Functional analysis of the Fusarium graminearum phosphatome. New Phytol 207:119–134. doi: 10.1111/nph.13374. [DOI] [PubMed] [Google Scholar]
- 45.Kim HK, Jo SM, Kim GY, Kim DW, Kim YK, Yun SH. 2015. A large-scale functional analysis of putative target genes of mating-type loci provides insight into the regulation of sexual development of the cereal pathogen Fusarium graminearum. PLoS Genet 11:e1005486. doi: 10.1371/journal.pgen.1005486. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 46.Liu H, Wang Q, He Y, Chen L, Hao C, Jiang C, Li Y, Dai Y, Kang Z, Xu JR. 2016. Genome-wide A-to-I RNA editing in fungi independent of ADAR enzymes. Genome Res 26:499–509. doi: 10.1101/gr.199877.115. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 47.Son H, Park AR, Lim JY, Shin C, Lee YW. 2017. Genome-wide exonic small interference RNA-mediated gene silencing regulates sexual reproduction in the homothallic fungus Fusarium graminearum. PLoS Genet 13:e1006595. doi: 10.1371/journal.pgen.1006595. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 48.Trail F, Common R. 2000. Perithecial development by Gibberella zeae: a light microscopy study. Mycologia 92:130–138. doi: 10.2307/3761457. [DOI] [Google Scholar]
- 49.Anavy L, Levin M, Khair S, Nakanishi N, Fernandez-Valverde SL, Degnan BM, Yanai I. 2014. BLIND ordering of large-scale transcriptomic developmental timecourses. Development 141:1161–1166. doi: 10.1242/dev.105288. [DOI] [PubMed] [Google Scholar]
- 50.Guenther JC, Hallen-Adams HE, Bücking H, Shachar-Hill Y, Trail F. 2009. Triacylglyceride metabolism by Fusarium graminearum during colonization and sexual development on wheat. Mol Plant Microbe Interact 22:1492–1503. doi: 10.1094/MPMI-22-12-1492. [DOI] [PubMed] [Google Scholar]
- 51.Weirick T, Militello G, Müller R, John D, Dimmeler S, Uchida S. 2016. The identification and characterization of novel transcripts from RNA-seq data. Brief Bioinform 17:678–685. doi: 10.1093/bib/bbv067. [DOI] [PubMed] [Google Scholar]
- 52.Wang L, Park HJ, Dasari S, Wang S, Kocher JP, Li W. 2013. CPAT: Coding-Potential Assessment Tool using an alignment-free logistic regression model. Nucleic Acids Res 41:e74. doi: 10.1093/nar/gkt006. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 53.Chakraborty S, Deb A, Maji RK, Saha S, Ghosh Z. 2014. LncRBase: an enriched resource for lncRNA information. PLoS One 9:e108010. doi: 10.1371/journal.pone.0108010. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 54.Nam JW, Bartel DP. 2012. Long noncoding RNAs in C. elegans. Genome Res 22:2529–2540. doi: 10.1101/gr.140475.112. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 55.Pauli A, Valen E, Lin MF, Garber M, Vastenhouw NL, Levin JZ, Fan L, Sandelin A, Rinn JL, Regev A, Schier AF. 2012. Systematic identification of long noncoding RNAs expressed during zebrafish embryogenesis. Genome Res 22:577–591. doi: 10.1101/gr.133009.111. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 56.Li H, Wang Y, Chen M, Xiao P, Hu C, Zeng Z, Wang C, Wang J, Hu Z. 2016. Genome-wide long non-coding RNA screening, identification and characterization in a model microorganism Chlamydomonas reinhardtii. Sci Rep 6:34109. doi: 10.1038/srep34109. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 57.Nyberg KG, Machado CA. 2016. Comparative expression dynamics of intergenic long noncoding RNAs in the genus Drosophila. Genome Biol Evol 8:1839–1858. doi: 10.1093/gbe/evw116. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 58.Neil H, Malabat C, d’Aubenton-Carafa Y, Xu Z, Steinmetz LM, Jacquier A. 2009. Widespread bidirectional promoters are the major source of cryptic transcripts in yeast. Nature 457:1038–1042. doi: 10.1038/nature07747. [DOI] [PubMed] [Google Scholar]
- 59.Pelechano V, Wei W, Steinmetz LM. 2013. Extensive transcriptional heterogeneity revealed by isoform profiling. Nature 497:127–131. doi: 10.1038/nature12121. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 60.Cabili MN, Trapnell C, Goff L, Koziol M, Tazon-Vega B, Regev A, Rinn JL. 2011. Integrative annotation of human large intergenic noncoding RNAs reveals global properties and specific subclasses. Genes Dev 25:1915–1927. doi: 10.1101/gad.17446611. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 61.Ulitsky I, Shkumatava A, Jan CH, Sive H, Bartel DP. 2011. Conserved function of lincRNAs in vertebrate embryonic development despite rapid sequence evolution. Cell 147:1537–1550. doi: 10.1016/j.cell.2011.11.055. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 62.Motamedi MR, Verdel A, Colmenares SU, Gerber SA, Gygi SP, Moazed D. 2004. Two RNAi complexes, RITS and RDRC, physically interact and localize to noncoding centromeric RNAs. Cell 119:789–802. doi: 10.1016/j.cell.2004.11.034. [DOI] [PubMed] [Google Scholar]
- 63.Bühler M, Verdel A, Moazed D. 2006. Tethering RITS to a nascent transcript initiates RNAi- and heterochromatin-dependent gene silencing. Cell 125:873–886. doi: 10.1016/j.cell.2006.04.025. [DOI] [PubMed] [Google Scholar]
- 64.Zhang K, Mosch K, Fischle W, Grewal SIS. 2008. Roles of the Clr4 methyltransferase complex in nucleation, spreading and maintenance of heterochromatin. Nat Struct Mol Biol 15:381–388. doi: 10.1038/nsmb.1406. [DOI] [PubMed] [Google Scholar]
- 65.Bayne EH, White SA, Kagansky A, Bijos DA, Sanchez-Pulido L, Hoe KL, Kim DU, Park HO, Ponting CP, Rappsilber J, Allshire RC. 2010. Stc1: a critical link between RNAi and chromatin modification required for heterochromatin integrity. Cell 140:666–677. doi: 10.1016/j.cell.2010.01.038. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 66.Dang Y, Cheng J, Sun X, Zhou Z, Liu Y. 2016. Antisense transcription licenses nascent transcripts to mediate transcriptional gene silencing. Genes Dev 30:2417–2432. doi: 10.1101/gad.285791.116. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 67.Park AR, Cho AR, Seo JA, Min K, Son H, Lee J, Choi GJ, Kim JC, Lee YW. 2012. Functional analyses of regulators of G protein signaling in Gibberella zeae. Fungal Genet Biol 49:511–520. doi: 10.1016/j.fgb.2012.05.006. [DOI] [PubMed] [Google Scholar]
- 68.Chen Y, Gao Q, Huang M, Liu Y, Liu Z, Liu X, Ma Z. 2015. Characterization of RNA silencing components in the plant pathogenic fungus Fusarium graminearum. Sci Rep 5:12500. doi: 10.1038/srep12500. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 69.Mercer TR, Gerhardt DJ, Dinger ME, Crawford J, Trapnell C, Jeddeloh JA, Mattick JS, Rinn JL. 2011. Targeted RNA sequencing reveals the deep complexity of the human transcriptome. Nat Biotechnol 30:99–104. doi: 10.1038/nbt.2024. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 70.Cabili MN, Dunagin MC, McClanahan PD, Biaesch A, Padovan-Merhar O, Regev A, Rinn JL, Raj A. 2015. Localization and abundance analysis of human lncRNAs at single-cell and single-molecule resolution. Genome Biol 16:20. doi: 10.1186/s13059-015-0586-4. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 71.ENCODE Project Consortium 2007. Identification and analysis of functional elements in 1% of the human genome by the ENCODE pilot project. Nature 447:799–816. doi: 10.1038/nature05874. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 72.van Bakel H, Nislow C, Blencowe BJ, Hughes TR. 2010. Most “dark matter” transcripts are associated with known genes. PLoS Biol 8:e1000371. doi: 10.1371/journal.pbio.1000371. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 73.Anderson DM, Anderson KM, Chang CL, Makarewich CA, Nelson BR, McAnally JR, Kasaragod P, Shelton JM, Liou J, Bassel-Duby R, Olson EN. 2015. A micropeptide encoded by a putative long noncoding RNA regulates muscle performance. Cell 160:595–606. doi: 10.1016/j.cell.2015.01.009. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 74.Bánfai B, Jia H, Khatun J, Wood E, Risk B, Gundling WE, Kundaje A, Gunawardena HP, Yu Y, Xie L, Krajewski K, Strahl BD, Chen X, Bickel P, Giddings MC, Brown JB, Lipovich L. 2012. Long noncoding RNAs are rarely translated in two human cell lines. Genome Res 22:1646–1657. doi: 10.1101/gr.134767.111. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 75.Gascoigne DK, Cheetham SW, Cattenoz PB, Clark MB, Amaral PP, Taft RJ, Wilhelm D, Dinger ME, Mattick JS. 2012. Pinstripe: a suite of programs for integrating transcriptomic and proteomic datasets identifies novel proteins and improves differentiation of protein-coding and non-coding genes. Bioinformatics 28:3042–3050. doi: 10.1093/bioinformatics/bts582. [DOI] [PubMed] [Google Scholar]
- 76.Wilson BA, Masel J. 2011. Putatively noncoding transcripts show extensive association with ribosomes. Genome Biol Evol 3:1245–1252. doi: 10.1093/gbe/evr099. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 77.Chew GL, Pauli A, Rinn JL, Regev A, Schier AF, Valen E. 2013. Ribosome profiling reveals resemblance between long non-coding RNAs and 5′ leaders of coding RNAs. Development 140:2828–2834. doi: 10.1242/dev.098343. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 78.Ingolia NT, Brar GA, Stern-Ginossar N, Harris MS, Talhouarne GJS, Jackson SE, Wills MR, Weissman JS. 2014. Ribosome profiling reveals pervasive translation outside of annotated protein-coding genes. Cell Rep 8:1365–1379. doi: 10.1016/j.celrep.2014.07.045. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 79.Juntawong P, Girke T, Bazin J, Bailey-Serres J. 2014. Translational dynamics revealed by genome-wide profiling of ribosome footprints in Arabidopsis. Proc Natl Acad Sci U S A 111:E203–E212. doi: 10.1073/pnas.1317811111. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 80.Ji Z, Song R, Regev A, Struhl K. 2015. Many lncRNAs, 5′UTRs, and pseudogenes are translated and some are likely to express functional proteins. eLife 4:e08890. doi: 10.7554/eLife.08890. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 81.Carlevaro-Fita J, Rahim A, Guigó R, Vardy LA, Johnson R. 2016. Cytoplasmic long noncoding RNAs are frequently bound to and degraded at ribosomes in human cells. RNA 22:867–882. doi: 10.1261/rna.053561.115. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 82.Kang YJ, Yang DC, Kong L, Hou M, Meng YQ, Wei L, Gao G. 2017. CPC2: a fast and accurate coding potential calculator based on sequence intrinsic features. Nucleic Acids Res 45:W12–W16. doi: 10.1093/nar/gkx428. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 83.Bogu GK, Vizán P, Stanton LW, Beato M, Croce LD, Marti-Renom MA. 2015. Chromatin and RNA maps reveal regulatory long noncoding RNAs in mouse. Mol Cell Biol 36:809–819. doi: 10.1128/MCB.00955-15. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 84.Wery M, Descrimes M, Vogt N, Dallongeville AS, Gautheret D, Morillon A. 2016. Nonsense-mediated decay restricts lncRNA levels in yeast unless blocked by double-stranded RNA structure. Mol Cell 61:379–392. doi: 10.1016/j.molcel.2015.12.020. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 85.Liu S, Wang Z, Chen D, Zhang B, Tian RR, Wu J, Zhang Y, Xu K, Yang LM, Cheng C, Ma J, Lv L, Zheng YT, Hu X, Zhang Y, Wang X, Li J. 2017. Annotation and cluster analysis of spatiotemporal- and sex-related lncRNA expression in rhesus macaque brain. Genome Res 27:1608–1620. doi: 10.1101/gr.217463.116. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 86.German MA, Pillay M, Jeong DH, Hetawal A, Luo S, Janardhanan P, Kannan V, Rymarquis LA, Nobuta K, German R, De Paoli ED, Lu C, Schroth G, Meyers BC, Green PJ. 2008. Global identification of microRNA-target RNA pairs by parallel analysis of RNA ends. Nat Biotechnol 26:941–946. doi: 10.1038/nbt1417. [DOI] [PubMed] [Google Scholar]
- 87.Cloutier SC, Ma WK, Nguyen LT, Tran EJ. 2012. The DEAD box RNA helicase Dbp2 connects RNA quality control with repression of aberrant transcription. J Biol Chem 287:26155–26166. doi: 10.1074/jbc.M112.383075. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 88.Cheng P, He Q, He Q, Wang L, Liu Y. 2005. Regulation of the Neurospora circadian clock by an RNA helicase. Genes Dev 19:234–241. doi: 10.1101/gad.1266805. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 89.Emerson JM, Bartholomai BM, Ringelberg CS, Baker SE, Loros JJ, Dunlap JC. 2015. period-1 encodes an ATP-dependent RNA helicase that influences nutritional compensation of the Neurospora circadian clock. Proc Natl Acad Sci U S A 112:15707–15712. doi: 10.1073/pnas.1521918112. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 90.Zofall M, Yamanaka S, Reyes-Turcu FE, Zhang K, Rubin C, Grewal SIS. 2012. RNA elimination machinery targeting meiotic mRNAs promotes facultative heterochromatin formation. Science 335:96–100. doi: 10.1126/science.1211651. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 91.Böhmdorfer G, Wierzbicki AT. 2015. Control of chromatin structure by long noncoding RNA. Trends Cell Biol 25:623–632. doi: 10.1016/j.tcb.2015.07.002. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 92.Ni T, Tu K, Wang Z, Song S, Wu H, Xie B, Scott KC, Grewal SI, Gao Y, Zhu J. 2010. The prevalence and regulation of antisense transcripts in Schizosaccharomyces pombe. PLoS One 5:e15271. doi: 10.1371/journal.pone.0015271. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 93.Rhind N, Chen Z, Yassour M, Thompson DA, Haas BJ, Habib N, Wapinski I, Roy S, Lin MF, Heiman DI, Young SK, Furuya K, Guo Y, Pidoux A, Chen HM, Robbertse B, Goldberg JM, Aoki K, Bayne EH, Berlin AM, Desjardins CA, Dobbs E, Dukaj L, Fan L, FitzGerald MG, French C, Gujja S, Hansen K, Keifenheim D, Levin JZ, Mosher RA, Müller CA, Pfiffner J, Priest M, Russ C, Smialowska A, Swoboda P, Sykes SM, Vaughn M, Vengrova S, Yoder R, Zeng Q, Allshire R, Baulcombe D, Birren BW, Brown W, Ekwall K, Kellis M, Leatherwood J, Levin H, Margalit H, Martienssen R, Nieduszynski CA, Spatafora JW, Friedman N, Dalgaard JZ, Baumann P, Niki H, Regev A, Nusbaum C. 2011. Comparative functional genomics of the fission yeasts. Science 332:930–936. doi: 10.1126/science.1203357. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 94.Zhang L, Ma H, Pugh BF. 2011. Stable and dynamic nucleosome states during a meiotic developmental process. Genome Res 21:875–884. doi: 10.1101/gr.117465.110. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 95.Chen HM, Rosebrock AP, Khan SR, Futcher B, Leatherwood JK. 2012. Repression of meiotic genes by antisense transcription and by Fkh2 transcription factor in Schizosaccharomyces pombe. PLoS One 7:e29917. doi: 10.1371/journal.pone.0029917. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 96.Cloutier SC, Wang S, Ma WK, Petell CJ, Tran EJ. 2013. Long noncoding RNAs promote transcriptional poising of inducible genes. PLoS Biol 11:e1001715. doi: 10.1371/journal.pbio.1001715. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 97.Cloutier SC, Wang S, Ma WK, Al Husini NA, Dhoondia Z, Ansari A, Pascuzzi PE, Tran EJ. 2016. Regulated formation of lncRNA-DNA hybrids enables faster transcriptional induction and environmental adaptation. Mol Cell 61:393–404. doi: 10.1016/j.molcel.2015.12.024. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 98.Ørom UA, Derrien T, Beringer M, Gumireddy K, Gardini A, Bussotti G, Lai F, Zytnicki M, Notredame C, Huang Q, Guigo R, Shiekhattar R. 2010. Long non-coding RNAs with enhancer-like function in human. Cell 143:46–58. doi: 10.1016/j.cell.2010.09.001. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 99.Wang KC, Yang YW, Liu B, Sanyal A, Corces-Zimmerman R, Chen Y, Lajoie BR, Protacio A, Flynn RA, Gupta RA, Wysocka J, Lei M, Dekker J, Helms JA, Chang HY. 2011. A long noncoding RNA maintains active chromatin to coordinate homeotic gene expression. Nature 472:120–124. doi: 10.1038/nature09819. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 100.Li W, Notani D, Ma Q, Tanasa B, Nunez E, Chen AY, Merkurjev D, Zhang J, Ohgi K, Song X, Oh S, Kim HS, Glass CK, Rosenfeld MG. 2013. Functional roles of enhancer RNAs for oestrogen-dependent transcriptional activation. Nature 498:516–520. doi: 10.1038/nature12210. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 101.Boque-Sastre R, Soler M, Oliveira-Mateos C, Portela A, Moutinho C, Sayols S, Villanueva A, Esteller M, Guil S. 2015. Head-to-head antisense transcription and R-loop formation promotes transcriptional activation. Proc Natl Acad Sci U S A 112:5785–5790. doi: 10.1073/pnas.1421197112. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 102.Bitton DA, Grallert A, Scutt PJ, Yates T, Li Y, Bradford JR, Hey Y, Pepper SD, Hagan IM, Miller CJ. 2011. Programmed fluctuations in sense/antisense transcript ratios drive sexual differentiation in S. pombe. Mol Syst Biol 7:559. doi: 10.1038/msb.2011.90. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 103.Bumgarner SL, Neuert G, Voight BF, Symbor-Nagrabska A, Grisafi P, van Oudenaarden A, Fink GR. 2012. Single-cell analysis reveals that noncoding RNAs contribute to clonal heterogeneity by modulating transcription factor recruitment. Mol Cell 45:470–482. doi: 10.1016/j.molcel.2011.11.029. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 104.Rosa S, Duncan S, Dean C. 2016. Mutually exclusive sense-antisense transcription at FLC facilitates environmentally induced gene repression. Nat Commun 7:13031. doi: 10.1038/ncomms13031. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 105.Li N, Joska TM, Ruesch CE, Coster SJ, Belden WJ. 2015. The frequency natural antisense transcript first promotes, then represses, frequency gene expression via facultative heterochromatin. Proc Natl Acad Sci U S A 112:4357–4362. doi: 10.1073/pnas.1406130112. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 106.Metzenberg RL. 2004. Bird medium: an alternative to Vogel medium. Fungal Genet Rep 51: doi: 10.4148/1941-4765.1138. [DOI] [Google Scholar]
- 107.Kim D, Langmead B, Salzberg SL. 2015. HISAT: a fast spliced aligner with low memory requirements. Nat Methods 12:357–360. doi: 10.1038/nmeth.3317. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 108.Pertea M, Pertea GM, Antonescu CM, Chang TC, Mendell JT, Salzberg SL. 2015. StringTie enables improved reconstruction of a transcriptome from RNA-seq reads. Nat Biotechnol 33:290–295. doi: 10.1038/nbt.3122. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 109.Anders S, Pyl PT, Huber W. 2015. HTSeq—a python framework to work with high-throughput sequencing data. Bioinformatics 31:166–169. doi: 10.1093/bioinformatics/btu638. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 110.Robinson MD, McCarthy DJ, Smyth GK. 2010. edgeR: a Bioconductor package for differential expression analysis of digital gene expression data. Bioinformatics 26:139–140. doi: 10.1093/bioinformatics/btp616. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 111.Law CW, Alhamdoosh M, Su S, Smyth GK, Ritchie ME. 2016. RNA-seq analysis is easy as 1-2-3 with limma, Glimma and edgeR. F1000Res 5:1408. doi: 10.12688/f1000research.9005.2. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 112.Bryant DM, Johnson K, DiTommaso T, Tickle T, Couger MB, Payzin-Dogru D, Lee TJ, Leigh ND, Kuo TH, Davis FG, Bateman J, Bryant S, Guzikowski AR, Tsai SL, Coyne S, Ye WW, Freeman RM Jr, Peshkin L, Tabin CJ, Regev A, Haas BJ, Whited JL. 2017. A tissue-mapped axolotl de novo transcriptome enables identification of limb regeneration factors. Cell Rep 18:762–776. doi: 10.1016/j.celrep.2016.12.063. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 113.Aslett M, Wood V. 2006. Gene Ontology annotation status of the fission yeast genome: preliminary coverage approaches 100%. Yeast 23:913–919. doi: 10.1002/yea.1420. [DOI] [PubMed] [Google Scholar]
- 114.Young MD, Wakefield MJ, Smyth GK, Oshlack A. 2010. Gene Ontology analysis for RNA-seq: accounting for selection bias. Genome Biol 11:R14. doi: 10.1186/gb-2010-11-2-r14. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 115.Wheeler TJ, Eddy SR. 2013. Nhmmer: DNA homology search with profile HMMs. Bioinformatics 29:2487–2489. doi: 10.1093/bioinformatics/btt403. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 116.Langfelder P, Horvath S. 2008. WGCNA: an R package for weighted correlation network analysis. BMC Bioinformatics 9:559. doi: 10.1186/1471-2105-9-559. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 117.Zhang B, Horvath S. 2005. A general framework for weighted gene co-expression network analysis. Stat Appl Genet Mol Biol 4: doi: 10.2202/1544-6115.1128. [DOI] [PubMed] [Google Scholar]
- 118.Lee HC, Li L, Gu W, Xue Z, Crosthwaite SK, Pertsemlidis A, Lewis ZA, Freitag M, Selker EU, Mello CC, Liu Y. 2010. Diverse pathways generate microRNA-like RNAs and Dicer-independent small interfering RNAs in fungi. Mol Cell 38:803–814. doi: 10.1016/j.molcel.2010.04.005. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 119.Shahid S, Axtell MJ. 2014. Identification and annotation of small RNA genes using ShortStack. Methods 67:20–27. doi: 10.1016/j.ymeth.2013.10.004. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 120.Dichtl B, Stevens A, Tollervey D. 1997. Lithium toxicity in yeast is due to the inhibition of RNA processing enzymes. EMBO J 16:7184–7195. doi: 10.1093/emboj/16.23.7184. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 121.Frazee AC, Pertea G, Jaffe AE, Langmead B, Salzberg SL, Leek JT. 2015. Ballgown bridges the gap between transcriptome assembly and expression analysis. Nat Biotechnol 33:243–246. doi: 10.1038/nbt.3172. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 122.Pertea M, Kim D, Pertea GM, Leek JT, Salzberg SL. 2016. Transcript-level expression analysis of RNA-seq experiments with HISAT, StringTie, and Ballgown. Nat Protoc 11:1650–1667. doi: 10.1038/nprot.2016.095. [DOI] [PMC free article] [PubMed] [Google Scholar]
Associated Data
This section collects any data citations, data availability statements, or supplementary materials included in this article.