Skip to main content

Advertisement

Quantitative analysis of cryptic splicing associated with TDP-43 depletion

BMC Medical Genomics volume 10, Article number: 38 (2017) Cite this article

Abstract

Background

Reliable exon recognition is key to the splicing of pre-mRNAs into mature mRNAs. TDP-43 is an RNA-binding protein whose nuclear loss and cytoplasmic aggregation are a hallmark pathology in amyotrophic lateral sclerosis and frontotemporal dementia (ALS/FTD). TDP-43 depletion causes the aberrant inclusion of cryptic exons into a range of transcripts, but their extent, relevance to disease pathogenesis and whether they are caused by other RNA-binding proteins implicated in ALS/FTD are unknown.

Methods

We developed an analysis pipeline to discover and quantify cryptic exon inclusion and applied it to publicly available human and murine RNA-sequencing data.

Results

We detected widespread cryptic splicing in TDP-43 depletion datasets but almost none in another ALS/FTD-linked protein FUS. Sequence motif and iCLIP analysis of cryptic exons demonstrated that they are bound by TDP-43. Unlike the cryptic exons seen in hnRNP C depletion, those repressed by TDP-43 cannot be linked to transposable elements. Cryptic exons are poorly conserved and inclusion overwhelmingly leads to nonsense-mediated decay of the host transcript, with reduced transcript levels observed in differential expression analysis. RNA-protein interaction data on 73 different RNA-binding proteins showed that, in addition to TDP-43, 7 specifically bind TDP-43 linked cryptic exons. This suggests that TDP-43 competes with other splicing factors for binding to cryptic exons and can repress cryptic exon inclusion.

Conclusions

Our quantitative analysis pipeline confirms the presence of cryptic exons during the depletion of TDP-43 but not FUS providing new insight into to RNA-processing dysfunction as a cause or consequence in ALS/FTD.

Open Peer Review reports

Background

Splicing depends on the reliable recognition and subsequent removal of non-coding intronic sequence by the multi-protein spliceosome complex. Boundaries that demarcate exons from introns are first recognised by the binding of the U1 small nuclear RNA (snRNA) to the 5′ splice site at the beginning of the intron and the U2 snRNA binding to the polypyrimidine tract and 3′ splice site at the end of the intron. The two snRNAs then interact with each other and the intronic sequence is removed via a series of transesterification reactions [1]. During splicing, regulatory sequences in the nascent RNAs recruit RNA-binding proteins (RBPs) to shape mRNAs, selecting or omitting particular exons by acting to enhance or repress splicing.

Due to the long length and reduced evolutionary conservation of intronic sequences, pairs of 3′ and 5′ splice sites can emerge randomly to create potentially new exons. These cryptic exons (also known as pseudoexons) arise due to mutations that create new splice sites or remove the existing binding sites for splicing repressors. These type of mutations have also been implicated in a number of genetic diseases [2,3,4,5]. Inclusion of a cryptic exon, untested by evolution, can destabilise the transcript or radically alter the eventual protein structure. The former can occur by the nonsense-mediated decay (NMD) pathway, which occurs when a transcript has a premature termination codon introduced either directly by the cryptic exon or by a subsequent shift of reading frame [6, 7].

Cryptic exons can also emerge from transposable elements. One such example are Alu elements, the predominant transposable element in primates which are often found within introns in the antisense direction [8]. The consensus Alu sequence consists of two arms joined by an adenine-rich linker ending with a poly-adenine tail. When transcribed in the antisense direction these uridine-rich sequences can act as cryptic polypyrimidine tracts and only a few mutations are required to convert them into viable exons in a process termed exonisation [9]. De novo mutations that lead to Alu exonisation have been found in a range of diseases [3, 4, 10, 11] suggesting a need for regulation of potentially damaging Alu exons. Alu exonisation is repressed by the RNA binding protein hnRNP C, which competes with the spliceosome component protein U2AF65, the partner of the U2 snRNA, for binding cryptic 3′ splice sites [12]. Due to the potentially negative effects of incorporation of new exons, aberrant recognition of cryptic exons needs to be repressed.

TDP-43 is an RNA-binding protein encoded by the TARDBP gene. Loss of TDP-43 from the nucleus accompanied by TDP-43 positive inclusions in the cytoplasm of cortical and spinal cord neurons is the hallmark pathology of amyotrophic lateral sclerosis (ALS) as well as the majority of cases of frontotemporal dementia (FTD) [13]. In addition, missense mutations in TARDBP can cause familial ALS [14]. These findings point to a central role of TDP-43 in the aetiology of ALS and FTD.

Rare ALS-causing mutations have been found in another RNA-binding protein, FUS [15] further raising the possibility that the impairment of RNA processing is a central cause of ALS. TDP-43 was first shown to repress the inclusion of exon 9 in the CFTR gene by binding to long UG-rich sequences [16] and subsequently shown to act as both a splicing enhancer and repressor [17,18,19]. TDP-43 and FUS have both been shown to bind a set of overlapping RNA targets [20]. Transcriptome-wide studies of the effects of TDP-43 depletion, overexpression or mutation have demonstrated widespread changes in gene expression and splicing [21,22,23,24]. Of particular interest are long intron containing genes, which are dramatically downregulated during both TDP-43 and FUS depletion [20, 23].

Recently, Ling and colleagues observed the inclusion of cryptic exons when TDP-43 was depleted in HeLa or mouse embryonic stem cells [25]. These cryptic exons were shown to originate from poorly evolutionarily conserved sequence and shared no positions between the two species. These findings raise the possibility that impaired exon recognition contributes to TDP-43’s role in ALS aetiology. We therefore aimed to replicate and expand the findings of Ling and colleagues. Firstly, we undertook a quantitative genome-wide analysis of cryptic exon patterns, defining objective criteria that take advantage of biological replicates when available. Secondly, we applied this computational strategy to seven datasets (four human and three murine models) to systematically quantify cryptic RNA alterations associated with depletion of TDP-43. In addition we also investigated FUS in order to determine whether modulation of cryptic splicing was a common feature of RBPs implicated in ALS. We also analysed hnRNP C, as it had been previously shown to repress cryptic exons. Lastly, we used independent protein-RNA interaction datasets, conservation data, repeat element annotation and splice site scoring to investigate the potential mechanisms linking TDP-43 depletion with the cryptic exon phenomenon.

Methods

Data preparation

Table 1 lists all the public data used in this study. For all RNA-seq data we first performed adapter and quality trimming (Phred score > 20) with Trim Galore (0.4.1) on the FASTQ files before aligning to either the human (hg38) or mouse (mm10) reference genome with STAR (2.4.2a) [26]. The resulting BAM file was sorted and PCR duplicate marked with NovoSort (1.03.09). Processed iCLIP peaks data was downloaded from the iCOUNT server (http://icount.biolab.si/). Both the human and mouse TDP-43 iCLIP data have been previously published [27, 28].

Table 1 List of accessions. For the ENCODE RNA-seq libraries, the control and target depletion samples are listed under separate accessions
Full size table

Processed eCLIP data (previously described by [29]) was downloaded from the ENCODE project. The narrowPeaks bed format was used with the first nucleotide of the cluster defined as the peak. Peak coordinates from iCLIP and eCLIP were converted to the hg38 and mm10 builds using the LiftOver tool from UCSC.

Cryptic splicing definition

Splicing aware alignment software such as STAR cut short reads that originate from a spliced transcript and align the pieces separately, marking the distance between them as a splice junction. Splice junctions can be used to reaffirm known splicing patterns or infer novel splicing. We define cryptic splicing as the emergence or relative increase in splice junctions that splice from known splice sites to unannotated positions within introns. This increase correlates with the depletion of a particular RNA binding protein. Different repositories have different levels of proof for annotating exons but we define an annotated exon as one listed in the Ensembl list of transcripts (release 82).

Cryptic splicing discovery with the CryptEx pipeline

Due to the diversity in the quality of published RNA-seq data, the cryptic splicing discovery pipeline was designed to be used on any RNA-seq library, whether single or paired end, stranded or unstranded, total RNA or polyA-selected RNA. However, when high quality RNA-seq data is available (paired end reads >100bp sequenced with >30M reads per sample), we instead suggest using one of the several recently released tools that can identify and classify unannotated splice junctions such as JunctionSeq [30], Leafcutter [31], MAJIQ [32] or SGSeq [33].

The inherent flexibility of our pipeline results in a large number of false positive hits which have to be aggressively filtered downstream. The initial cryptic exon discovery pipeline was written in Bash, using SAMTools (version 1.2) [34] and BEDTools (version 2.25.0) [35]. The statistical testing for differential cryptic exon usage was carried out using the well-known DEXSeq framework [36]. All code for downstream processing and filtering of cryptic hits was written in the R language (version 3.1.1) using the Biostrings, data.table, DEXSeq, dplyr, GenomicRanges, ggplot2, gridExtra, optparse, plyr, stringr, and tidyr packages. All the code for reproducing this paper is available in a GitHub repository [37].

In order to discover all possible splice junctions that travel into the intron we first extracted all spliced reads from each aligned bam file using SAMTools, filtering out any secondary alignments. To extract only the spliced reads that overlap an annotated exon we then performed an intersection in BEDTools with a flattened list of exons, created using the dexseq prepare annotation.py Python script included with the DEXSeq package [36]. An inverse intersection was then performed with the same exon list to retain only the spliced reads which do not bridge two annotated exons. The intronic mapping sections of each read were split off from the rest and retained. In each dataset all intronic mapping spliced reads from each sample were grouped together irrespective of condition. Split reads that were within 500bp of each other were merged into larger intervals, hereby referred to as tags. This ideally captures both the upstream and downstream splice junction to a central cryptic cassette exon. To keep only the tags that are splicing within the gene body another intersection was performed with a list of introns. This was generated from the same flattened exon file by an R script written by Devon Ryan [38]. The tags were then incorporated into the flattened list of exons. The reads that overlap annotated exons and tags were counted using HTSeq [39] on the default settings, ignoring PCR duplicate reads. The read counts were used to calculate differential usage of each exon with DEXSeq.

All the cryptic tags with an adjusted P-value (false discovery rate) < 5% and a | log2(fold change)| > 0.6 were extracted from the DEXSeq results table (see Additional file 1: Figure S1). The splice junctions from the alignment of each sample were used to work out the coordinates of the canonical junction that spans the intron within which the cryptic tag is or isn’t spliced in control samples. Using splice junctions from the depletion condition samples, the upstream and downstream junctions that connect the adjacent annotated exons to the cryptic tag were re-discovered and quantified. Any cryptic example that did not have at least one upstream or downstream junction per sample or had fewer than ten canonical splice junctions was removed. These junctions were used to calculate per-condition mean Percent Spliced In (PSI) values which are a ratio of cryptic splicing over the sum of cryptic and canonical splicing [40]. As a number of cryptic splicing events are present at a low level in control samples, ∆PSI values were created for both upstream and downstream splicing for each tag. This is the difference in PSI between the depletion samples and the control samples. Any cryptic tag that had either an upstream or downstream ∆PSI < 5% was removed.

iCLIP/eCLIP enrichment

The coordinates of each cryptic tag were flanked by 100 base pairs on either side to capture binding around the putative splice sites. In order to compare the overlap between cryptic exons and RNA-protein binding peaks, two sets of null exons were created for comparison, which maintain the same length as their corresponding cryptic exon but sample either the intronic sequence outside of the flanked exon or that of the adjacent introns within the same gene if available. Overlaps between exons and iCLIP and eCLIP peaks were calculated using BedTools.

Motif enrichment analysis

FASTA sequence was generated for the cryptic exons flanked by 100 nucleotides either side and submitted to the MEME web tool [41] under the default settings. The analysis was repeated using the HOMER algorithm [42] on RNA mode. Motifs were created using WebLogo [43]. Frequencies of the 16 possible dinucleotides were compared between flanked cryptic exon sequences with adjacent intron sequences from the same gene.

Transposable element enrichment

Lists of transposable elements in human and mouse (hg38 and mm10 respectively) were previously generated by the RepeatMasker tool [44] and were downloaded from UCSC. Overlap between different transposable elements and the cryptic exons was calculated in each orientation using BedTools.

Conservation analysis

PhyloP compares the sequence alignments of multiple species to produce per base conservation scores [45]. Average conservation score per cryptic tag was calculated using bigWigSummary (UCSC) for both human and mouse data. The lists of splice junctions created by STAR when aligning each sample were used to identify the coordinates of the exons adjacent to the cryptic exon. The randomly sampled intronic sequence from the cryptic-containing intron was used as a negative control.

Differential expression

For each sample the number of reads overlapping each gene were counted using HTSeq using the same Ensembl gene models as before. Differentially expressed genes were identified using DESeq2 [46] at a false discovery rate of 10%.

Protein prediction analysis

Any cryptic exon which did not fall within the coding sequence of a transcript was omitted. Splice junctions generated by STAR were used to determine the upstream and downstream exons adjacent to each cryptic exon. Only cryptic exons that had both upstream and downstream splice junctions (cassette exons) were kept. The upstream and downstream exons were matched to their corresponding annotated exon in the Ensembl transcript file for each species to assign the correct reading frame for translation. Nucleotide sequences for transcripts either including or excluding the central cryptic exon were created and translated in silico using the R Biostrings package. Premature termination codons (PTCs) were identified from the translated sequence and defined as escaping nonsense mediated decay (NMD) if they occurred within 50 nucleotides of the downstream exon-exon junction. Frameshifts were identified by comparing the sequence of the downstream exon with and without the central cryptic exon. A null distribution of PTC-containing or frame shifted transcripts was created by generating central exons from random nucleotide sequence, keeping the length distribution the same. For each species this was repeated 100 times.

Splice junction scoring

The strength of 5′ and 3′ splice sites was calculated for the human cryptic exons using maxEnt [47]. Higher scores indicate the increased log odds of a given splice site being a true splice site. The 5′ splice site is defined as the last 3 nucleotides of the upstream exon flanked by 6 intronic nucleotides, of which the first two are invariably GU. The 3′ splice site is defined as the last 20 intronic nucleotides of which the final two are invariably AG, flanked by the first 3 nucleotides of the downstream exon. The splice sites of annotated exons were used as a positive control. Randomly generated sequence with invariant AG or GT was used as a negative control. Paired t-tests were carried out to test the direction of change between the cryptic and annotated splice sites for each class of cryptic exon.

Results

Depletion of TDP-43 but not FUS results in cryptic exons

We compared the involvement of two ALS-linked RNA-binding proteins in cryptic splicing: TDP-43 and FUS. We analyzed publicly available TDP-43 depletion RNA-Seq datasets (three human, three murine, datasets 1–6 in Table 2), FUS depletion RNA-Seq datasets (1 human, 1 murine, datasets 7–8 in Table 2) and as a positive control a human hnRNP C depletion dataset for which cryptic exons have previously been reported (dataset 9 in Table 2). While these datasets differ in library preparation method, read depth and length, and protein depletion method (Table 2), the FUS datasets match the TDP-43 datasets in cell type, depletion method sequencing depth and lab of origin (Table 2), as do the TDP-43 and FUS depletion data created by the ENCODE consortium. Using these datasets, we took a genome-wide approach to describe the pattern of unannotated splicing in human and mouse that we call CryptEx. The first step involves identifying novel splice junctions between annotated exons and unannotated intronic regions. These reads were clustered to create putative cryptic exons. Making use of biological replicate samples we compared the abundance of reads covering the cryptic region relative to the rest of the annotated exons of the surrounding gene. Differential usage of each cryptic region was tested between depletion and control samples. Results were omitted if they fell outside of a strict 5% false discovery rate.

Table 2 All RNA-sequencing data used in this study
Full size table

In order to further refine our cryptic exon detection algorithm, we then measured the amount of splicing to and from each region and used this information to filter and classify cryptic splicing events into three categories of cryptic exon: (i) cassette-like, where novel 3′ and 5′ splice sites are recognised, which forms a completely new exon; (ii) 5′ extension, where a novel 3′ splice site is recognised and an existing exon is extended upstream of its annotated start and (iii) 3′ extension, where a novel 5′ splice site is recognised and an exon is extended downstream of its annotated end (Fig. 1a). Note that our approach does not consider fully retained introns, but several other methods have been designed for this purpose [48,49,50,51].

Fig. 1
figure1

Cryptic splicing discovered by the CryptEx pipeline. a Schematic of the three classes of cryptic exon. Black boxes represent annotated exons and red boxes represent a cryptic exon. Grey lines represent the spliced intron. b Tally of the three classes of cryptic exon discovered by the CryptEx pipeline across the nine datasets. “Unfiltered output” refers to the number of differentially used cryptic splicing events at a false discovery rate (FDR) < 5% before undergoing cryptic exon classification. Counts from Ling et al’s data are taken from the paper itself. c Venn diagrams showing the overlap between the six TDP-43 depletion datasets

Full size image

Figure 1b lists the counts of both pre-classification cryptic regions (“unfiltered output”) and the post-classification cryptic exons. Comparing the two human ENCODE K562 cell line TDP-43 depletion datasets (3-4), the poly-A selected mRNA-Seq dataset yielded far more splicing events than the total RNA dataset, presumably due to polyA selection leading to a higher coverage of mature spliced mRNA species. In total 95 human cryptic exons were discovered and classified, with the majority only detected in the mRNA-seq dataset. 11 cryptic splicing events were shared between datasets 3 and 4 (Fig. 1c). Of the 26 human cryptic exons reported by Ling, 12 were seen in at least one of the two datasets 3 and 4.

Both mouse datasets differ in both cell type (adult striatum in dataset 5 vs embryonic stem (ES) cell in dataset 6) and read depth (35-60M in dataset 5 vs 2-10M in dataset 6). 52 cryptic exons were identified in total, with 46 detected in the adult striatum and 15 in ES cells, with 6 exons observed in both. Of the 46 cryptic splicing events identified in murine samples by Ling et al, 13 were detected in at least one of datasets 5 and 6. Side by side visual inspection (Additional file 2: Figure S2 and Additional file 3: Figure S3) suggests that differences in library preparation and read depth are behind the low concordance rates in both human and mouse, as cryptic exons detected in the higher depth dataset (K562 mRNA and mouse adult brain) can be observed by eye in the lower depth dataset (K562 total RNA and mouse ES cell). These exons currently fail to be detected by the CryptEx algorithm.

No cryptic splicing events were shared between human and mouse as previously reported [25]. Note that to report overlap with Ling and colleagues (datasets 1 and 2), the raw data was unsuitable for our cryptic exon discovery pipeline due to a lack of biological replicate samples. Instead the sequence data was aligned and the splice junctions generated by the aligner were used to classify previously reported cryptic exons.

In contrast, while a large number of novel splicing events were observed in the FUS depletion datasets, our algorithm only classified 3 in mouse and 1 in human as cryptic exons. FUS depletion was not observed to produce any cassette-like cryptic exons in either species. Additional file 1: Figure S1 visualises the full unclassified output of the pipeline and illustrates the diversity of splicing alterations that occur upon RBP depletion. Additional file 2: Figure S2 and Additional file 3: Figure S3 comprise of screenshots of every reported cryptic exon from the IGV browser in mouse and human respectively. Additional file 4: Tables S1 and S2 (ST1/ST2) list the coordinates of each cryptic exon along with the results of each experiment.

To verify that the cryptic exons were not included under normal conditions, we looked for evidence of the 52 total mouse cryptic exons in a set of 9 mouse tissues previously published in [52]. For the 95 total human cryptic exons we looked for evidence of inclusion in 49 normal human tissues collected by the GTEx project [53]. For each cryptic exon we looked for junctions that splice to and from the cryptic exon and divided by the counts of a junction that spans the length of it, to produce a ratio of cryptic exon inclusion. Only 4 mouse and 3 human cryptic exons showed any evidence of being included at all in normal tissues, albeit at low levels and with very high variability (Additional file 5: Tables S5 and S6). This suggests that the cryptic exons we discovered are generally not included in normal tissues and that they can only be seen during the depletion of TDP-43.

Cryptic exons are enriched in TDP-43 binding motifs and iCLIP peaks

For the remainder of our study, cryptic exons were grouped into unions of all cassette-like exons and extension events discovered in human and mouse, totalling 95 human and 52 murine cryptic exons. We then explored whether TDP-43 binding could explain the observed splicing changes in RNA-Seq data, as observed by Ling and colleagues. We took two complementary and genome-wide approaches: (i) searching for enriched motifs in the RNA sequence including and surrounding the cryptic exons and (ii) correlating the positions of cryptic exons with TDP-43 protein-RNA interaction data.

TDP-43 can repress or enhance the inclusion of a given exon by either binding within or adjacent to the exonic sequence [27]. Hence for our motif search, we flanked cryptic exon sequences by 100 nucleotides on either side. UG-rich motifs were found to be enriched in both mouse and human cryptic exons using two different algorithms: MEME (Fig. 2a) and HOMER (Additional file 6: Figure S4). Of the 52 mouse cryptic exons 29 had a run of UG up to 40 nucleotides in length. Similarly, human cryptic exons were enriched in a UG motif but not in a continuous manner. By comparing the frequencies of 16 possible dinucleotides between the flanked cryptic exon sequence and the sequence of the adjacent intron either up or downstream of the cryptic-containing intron we were able to resolve the enrichment of UG dinucleotides (Fig. 2b). UG and GU were enriched in flanked cryptic exon sequence in both human (fold change GU = 1.53; UG = 1.48; P < 10−50; proportion test) and mouse (fold change GU = 2.14; UG = 1.85; P < 10−50; proportion test).

Fig. 2
figure2

Evidence of TDP-43 binding cryptic exons. a Results of MEME motif search. Only the motif with the greatest enrichment compared to background sequence is presented. b Dinucleotide enrichment in the flanked cryptic exons compared to adjacent introns. c Schematic of iCLIP peak enrichment test. For illustration a cassette-like cryptic exon (green box) is shown between two annotated exons (black boxes) separated by intronic sequence (black lines). The proportion of the group of cryptic exons flanked either side by 100 nucleotides (orange) that overlap at least one iCLIP peak is compared to the proportion of overlaps in a group of length matched sequences from either the surrounding intron (yellow) or an adjacent intron (blue) each randomly sampled 100 times per gene. d iCLIP peak overlap enrichment for the 95 human cryptic exons found in either K562 cell TDP-43 depletion dataset and the 52 cryptic exons found in either mouse TDP-43 depletion dataset. Error bars denote 95% confidence intervals of the binomial distribution. ∗ P < 0.05, ∗∗ P < 0.001, ∗∗∗ P < 10−16. All P-values adjusted for multiple testing by Bonferroni method

Full size image

Individual nucleotide resolution UV crosslinking followed by immunoprecipitation (iCLIP) allows for precise nucleotide-resolution observation of which RNA species interact with a particular RNA-binding protein [12, 54]. We downloaded all publicly available TDP-43 iCLIP data from the iCount repository (http://icount.biolab.si/). We then intersected each set of iCLIP peaks with our cryptic exons, surrounded by 100 base pairs of flanking sequence either side. The proportion of overlapping cryptic exons was compared to the proportion of overlap between iCLIP peaks and two classes of null exon; the first created from the surrounding intronic sequence outside of each flanked cryptic and the second from an adjacent intron (Fig. 2c). If TDP-43 binding was uniform throughout an intron or gene then we would expect to see similar proportions of overlap in each. However, both species show an enrichment in TDP-43 binding peaks specific to the cryptic exons in every iCLIP dataset used, with as much as 25% of human cryptic exons and 50% of mouse cryptic exons overlapping at least one iCLIP peak each (Fig. 2d; both species P < 10−16; proportion test).

Cryptic exons are marginally enriched in transposable elements

Motivated by previous findings of cryptic exons associated with hnRNP C depletion and caused by exonisation of antisense Alu elements [12, 55], we investigated whether TDP-43 induced cryptic exons preferentially overlap specific families of transposable elements and/or class of repetitive sequences. Transposable/repeat element annotations were obtained using the RepeatMasker software and these features were split by family and orientation. Although Alu elements are a subfamily within the primate SINE element family, we included them separately given the prior hnRNP C result. As transposable elements are abundant in the genome, the number of overlapping exons was compared as before to the overlap in the whole intron and adjacent introns.

The mouse cryptic exons show a modest enrichment in antisense SINE elements in and around the cryptic exons when compared to the rest of the surrounding intron. However the elements are also common in adjacent introns and so are not enriched for this comparison (Fig. 3a). The antisense SINE elements are mainly from the B2 family (Additional file 7: Table S3) which in the antisense direction is rich in stretches of UG dinucleotides (Additional file 7: Figure S5). Mouse cryptic exons are also enriched in repeat elements annotated as “low complexity” or “simple repeat”, which are also mostly UG dinucleotide repeats, labelled as such or as AC repeats antisense to the direction of transcription. The human cryptic exons only show a small enrichment in”simple repeat” elements (Fig. 3b), most of which contain sense UG or antisense AC repeats (Additional file 7: Table S4). This contrasts with hnRNP C depletion, which shows a striking enrichment of antisense SINE elements of which all are of the Alu type (P < 10−16; proportion test), a result consistent with previous analyses of dataset 9 [12]. Altogether, these results are in line with findings from the motif analysis, that cryptic exons are enriched in TDP-43 binding motifs but not due to the large - scale enrichment in transposable elements.

Fig. 3
figure3

Cryptic exons in transposable elements Overlap between different families of repetitive element with lists of exons, separated by orientation. a Mouse TDP-43 depletion. b Human TDP-43 depletion. c Human hnRNP C depletion. The proportion of the cryptic exons that contain a particular element are shown in orange. Length - matched random samples from the surrounding intron (yellow) and adjacent introns (blue) are used as controls. LINE: Long Interspersed Nuclear Element; SINE: Short Interspersed Nuclear Element. ∗ : P < 0.05, ∗∗ : P < 0.001, ∗∗∗ : P < 10−16 . All P-values corrected for multiple testing with Bonferroni method

Full size image

Cryptic exons are poorly conserved and their inclusion acts to destabilise their host transcript

We then quantified the extent of evolutionary conservation of cryptic exons using the multiple species alignment conservation scores generated by PhyloP. We calculated mean conservation scores per exon for the cryptic exons and compared them to scores from both the annotated exons and randomly sampled intronic sequences from the same genes. We found no difference between cryptic exons and matched intronic sequences (Fig. 4a), and a much lower conservation level than adjacent annotated exons.

Fig. 4
figure4

Conservation and premature termination codon analysis. a Per exon average PhyloP conservation scores in cryptic exons, adjacent exons within the same set of genes (when available) and randomly sampled sequences from the cryptic containing intron. Box plots show first quartile, median and third quartile with the notches representing the 95% confidence interval of the median. Whiskers represent the minimum and maximum values that fall within 1.5 times the interquartile range. b The functional impact of cryptic exon inclusion on the host transcripts in human and mouse. Colours indicate the category of prediction and box size indicates the proportion of the total group of exons in each category. Categories from top to bottom: Frame shifted (red); Frame shifted and at least one premature termination codon (PTC) included (orange); PTC included only (yellow); Frame shifted but the resulting PTC falls within 50bp of the exon-exon junction, creating a truncated protein of novel sequence (light blue); PTC falls within 50bp of the exon-exon junction, creating a truncated protein (dark blue); Frame shift without any PTCs to create a protein of novel sequence (light green); Cryptic exon inclusion does not frame shift nor introduces a PTC, behaving as a benign cassette exon (dark green). For each species there is a corresponding set of predictions calculated from random sequences with matching lengths

Full size image

We also investigated the consequences of inclusion of cryptic exons on translation of the transcript. The inclusion of a premature termination codon (PTC) into a transcript could lead to either mRNA degradation by the nonsense-mediated decay (NMD) pathway. Alternatively, if the PTC falls within 50 nucleotides upstream of an exon-exon junction then NMD can be evaded, leading to the production of a truncated protein [7]. These two outcomes are compounded by the possibility of a cryptic exon shifting the reading frame of the downstream exon, leading either to more PTCs or the creation of a benign transcript of a different function. This gives cryptic exon inclusion six functional outcomes that can destabilise either the RNA or the downstream protein. We tested for all these outcomes by translating the predicted transcripts in silico. In this analysis we only considered the”cassette-like” cryptic exons that had both upstream and downstream splice junctions. Of the 31 human cryptic exons tested, 21 (67%) are predicted to destabilise their host transcript through the NMD pathway (Fig. 4b). Five cryptic exons are predicted to impart new functionality whereas five others are predicted to contain premature stop codons but evade NMD, creating truncated proteins upon translation. However, comparing these results to randomly generated sequence of the same length demonstrates that this distribution of outcomes can occur purely by chance. The 23 mouse cryptic exons tested behave similarly, with four cryptic exons creating functional proteins, one creating a new downstream protein, six leading to protein truncation and 12 being degraded by NMD (Fig. 4b). The random sequences were similarly distributed. Together this suggests that the cryptic exons are not enriched in particular sequence features and upon inclusion behave like randomly chosen sequences. This disruption of multiple mRNA species may have an effect at the protein level and explain the toxicity seen in response to TDP-43 depletion.

Cryptic exon containing genes are downregulated

We then investigated, in datasets 3-6, whether genes containing cryptic exons showed a specific pattern of altered expression. We calculated the proportion of the cryptic exon containing genes in each dataset that were differentially expressed at a FDR of 10%. We compared this with the proportion of differential expression of all genes with an expression level at or greater than the lowest expressed cryptic exon found in that dataset. Figure 5a shows the number of differentially expressed genes in each dataset as a proportion of the total, separated by direction. In all four TDP-43 depletion datasets, the cryptic exon containing genes as a group are more likely to be significantly downregulated compared to the genome-wide proportion (P < 0.001; hypergeometric test).

Fig. 5
figure5

Differential expression of cryptic exon genes. a Significantly differentially expressed genes between TDP-43 depletion and control samples (false discovery rate = 10%) in datasets 3-6. Comparisons were made between all genes tested with an expression level at or greater than the lowest expressed cryptic exon (“all genes”) and the genes where cryptic exons were discovered (“cryptic exon genes”) with each group divided by direction of change. b As above but for cryptic exon genes from the other dataset of the same species. Error bars show 95% confidence intervals for each proportion. ∗ : P < 0.05, ∗∗ : P < 0.001. All P-values adjusted by Bonferroni correction

Full size image

Furthermore, we performed the same analysis for each dataset with the cryptic exon containing genes that were only found in the other dataset of the same species (Fig. 5b). Surprisingly, in the mouse ES cell dataset 6 there was an enrichment of downregulated genes that contain cryptic exons only detectable in the mouse adult brain dataset 5 (P < 0.001; hypergeometric test). Visual inspection of these 10 introns in the mouse ES cell data (Additional file 2: Figure S2) suggests that seven of them may harbour cryptic exons in the ES cell data that are currently undetectable by the CryptEx algorithm.

Human cryptic exons are driven by the recognition of strong splice sites that are normally repressed

Whereas cassette-like cryptic exons appear as separate exons distinct from their surrounding exons, extension events must rely on a switch from a canonical splice site to a newly accessible splice site. We hypothesised that these extension events result from competition between two splice sites upon TDP-43 depletion. This would require the sequence of and around the cryptic splice site to be similarly recognisable to the spliceosome. Using the MaxEnt statistical model [47] to score splice sites by comparing their DNA sequences with constitutive observed canonical sequences, we scored the 5′ and 3′ splice sites of our cryptic exons and compared them with the scores of the surrounding canonical splice sites. The model compares splice sites from annotated exons with so-called decoy splice sites that retain the consensus AG/GT at the 3′ or 5′ splice site respectively. Therefore we also scored randomly generated sequences, which retained the consensus AG/GT positions. Figure 6 shows the scores for both the 3′ and 5′ splice sites for each class of human cryptic exons. Although the canonical splice sites were on average stronger than their corresponding cryptic splice site (P < 0.05; paired t-test), the majority had scores far greater than those from random sequence, suggesting that they are able function as real, albeit weaker, splice sites when TDP-43 is depleted.

Fig. 6
figure6

Scoring cryptic splice sites against canonical splice sites. Cassette-like cryptic exons have 5′ and 3′ splice sites that are recognised by the spliceosome under TDP-43 depletion. 5′ and 3′ splice site scores are plotted separately. Cryptic splice sites are shown in red, canonical splice sites are shown in blue. Random sequences with AG or GT consensus are plotted in grey. Cryptic extensions are the result of a cryptic splice site competing with the canonical splice site. 5′ extensions result from cryptic 3′ splice sites whereas 3′ extensions result from cryptic 5′ splice sites. Box plots show first quartile, median and third quartile with the notches representing the 95% confidence interval of the median. Whiskers represent the minimum and maximum values that fall within 1.5 times the interquartile range. Outliers are plotted as black dots. Cryptic splice sites are compared to canonical splice sites with paired t-tests. ∗ : P < 0.05, ∗∗ : P < 0.001

Full size image

Cryptic exons are bound by other RNA - binding proteins

Proteomic studies have demonstrated that TDP-43 interacts with a number of RNA-binding proteins (RBPs), including multiple members of the heterologously expressed ribonucleoprotein (hnRNP) family and other splicing factors [56,57,58]. The splicing of specific annotated exons has been shown to depend on the interaction of TDP-43 with multiple splicing factors [59]. We hypothesised that some cryptic exons may be included indirectly through a loss of TDP-43’s interactions with different RBPs. Van Nostrand and colleagues have performed eCLIP, a higher throughput modification of the iCLIP protocol, on 73 different RBPs including TDP-43 and FUS [29]. The experiments were carried out in two human cell lines (K562 and HepG2) with 29 of the RBPs being tested in both cell lines. We performed the same overlap analysis between our human cryptic exons and each set of eCLIP peaks, using the same two sets of control sequences as before. Each eCLIP experiment was performed in duplicate. This gives each RBP four possible enrichment results using a proportion test. For each RBP, the highest P-value from the four tests was reported and corrected for multiple testing using a strict Bonferroni approach. Only proteins with a resulting P < 0.05 are reported. Unsurprisingly TDP-43 had the highest number of overlapping exons (P < 10−22; proportion test), followed by U2AF65, TIA1, SRSF7, U2AF35, PPIG, SRSF1 and IGF2BP1. Figure 7a shows the overlap between the different RBPs and the human cryptic exons. Figure 7b shows the overlap between each gene (columns) against each RBP (rows). Hierarchical clustering was performed on the RBPs. The three largest clusters consist of TDP-43 alone, the U2 snRNP binding proteins U2AF35 and U2AF65, and a third cluster containing the other proteins.

Fig. 7
figure7

Mining of ENCODE eCLIP data in K562 and HepG2 cells. a RNA-binding proteins (RBPs) with significant (P < 0.05) proportion of overlapping cryptic exons (red) compared to sampled intronic sequence from the same (green) and adjacent introns (blue). b Comparison of eCLIP datasets from different RNA binding proteins (columns) showing the overlap with the cryptic exons (rows). RBPs in bold typeface are from K562 cells whereas those in regular typeface are from HepG2 cells

Full size image

Discussion

We have designed an analytical strategy to identify cryptic splicing that takes advantage of biological replicates in RNA sequencing data. We have applied this tool to a set of human and murine TDP-43 depletion datasets, as well as datasets that deplete hnRNP C or FUS. Our results are consistent with the previous findings that depletion of TDP-43 or hnRNP C leads to the inclusion of novel cryptic exons in both human and mouse, albeit with hnRNP C depletion leading to a far greater number of events than TDP-43. Although FUS undoubtedly plays an important role in splicing and mRNA stability and shares a number of targets with TDP-43 [20], the low number of cryptic exons observed due to FUS depletion suggests that it does not play a major role in cryptic splicing and is a key point of differentiation with TDP-43. This is despite the FUS and TDP-43 data analysed being produced under the same conditions for both mouse and human.

Further examination of TDP-43 linked exons suggests they tend to possess the necessary UG-rich sequence elements to be bound by TDP-43 and using iCLIP data we observed that a subset of the cryptic exons are bound by TDP-43 in vivo. We went on to investigate the origins of these TDP-43 bound cryptic exons, as has been done for the targets of hnRNP C. We observed that unlike hnRNP C linked cryptic exons, which invariably originate from antisense Alu elements, TDP-43 linked cryptic exons do not originate from any single family of transposable element. Furthermore their sequences show very low species conservation, akin to random intronic sequence, but remarkably they contain splice sites very close in strength to those of their adjacent annotated exons. Our differential expression analysis suggests that the bulk of cryptic exon containing genes are significantly downregulated upon TDP-43 depletion. We hypothesize that while some cassette-like cryptic exons will create functional or truncated proteins, most will lead to premature stop codons and nonsense-mediated decay of the inclusion transcript. The large number of exon extensions discovered by CryptEx may similarly lead to frameshifting and nonsense-mediated decay upon inclusion but may alternatively be sequestered in the nucleus and degraded by the mRNA surveillance pathway, as has been observed for retained introns [60]. A number of cassette-like cryptic exons could be not be spliced in silico to any annotated coding exons, suggesting a role for cryptic exon inclusion in to upstream open reading frames and 3′ untranslated regions, both of which have been observed to provide a site for modulation of gene expression by introducing premature termination codons [61, 62].

Consistent with this possibility, a recent proteomic study of TDP-43 depletion in human SH-SY5Y cells [63] that protein levels were changed for 3 of the 95 human cryptic exon containing genes. Two, HUWE1 and GOLGB1 had protein levels that were 8 and 31% of the control cells respectively whereas the third, HNRNPH3 was found to be 7-fold increased under TDP-43 depletion. Interestingly, the cryptic exon discovered in HNRNPH3 falls upstream of the start codon whereas those found in HUWE1 and GOLGB1 are predicted to trigger NMD by inclusion into the coding sequence (see Additional file 4: Table S1). Another gene with cryptic splicing seen in both K562 datasets and in the initial Ling HeLa data, AGRN, was recently shown to be decreased at the protein level in the cerebrospinal fluid of ALS patients compared to healthy controls and other neurological diseases [64]. Correct splicing of AGRN has shown to be crucial for the formation of the neuromuscular junction [65].

Our current understanding of TDP-43’s role in cryptic splicing is that of a safeguard against the inclusion of potentially damaging intronic sequence into transcripts. However, the relationship between the UG-rich sequences and the strong 5′ and 3′ splice sites and their changes over evolutionary time are unknown as we observed no conserved cryptic exons between human and mouse.

Using publicly available ENCODE eCLIP data, we identified a number of RNA binding proteins that also bind subsets of human cryptic exons under normal conditions, that is, in the presence of TDP-43. It is unsurprising that the splicing factors U2AF35 and U2AF65 are enriched as they preferably bind pyrimidine-rich 3′ splice site sequences, which all cryptic exons appear to possess. That only 10–15% of cryptic exons show U2AF35/65 binding may be due to competition from TDP-43 in a manner similar to that seen between hnRNP C and U2AF65. TIA-1 is an exciting finding due to its role in the formation of stress granules, key regulators of RNA stability [66]. In addition, IGF2BP1 has been reported as binding to TDP-43 in HEK293T and HeLa cell extracts [57, 58], whereas SRSF7 was reported as binding to TDP-43 in mouse N2A cells [56]. None of the observed proteins have been reported to change their protein level in response to TDP-43 depletion [63].

As the majority of cryptic exons are predicted to lead to nonsense-mediated decay of the inclusion transcript it seems peculiar that we can observe these transcripts at all. We hypothesise that cryptic splicing may be much more widespread than can be observed by RNA sequencing due to the highly efficient nature of nonsense- mediated decay. Over half of all cryptic exon genes are significantly downregulated in each dataset (Fig. 2b), suggesting that cryptic exon inclusion may be a key mechanism in the widespread changes in RNA expression that occur upon TDP-43 depletion. An alternative hypothesis is there is an interaction between TDP-43 and hnRNPC with the NMD machinery, which reduces the efficiency of degradation that is not shared by FUS. Experiments depleting both hnRNP C and the NMD component UPF1 have increased the number of hnRNP C-associated cryptic exons even further [67], suggesting that these experiment should be repeated for TDP-43 and FUS to better understand the relationship between cryptic splicing and mRNA degradation. Differences between the number of cryptic exons between TDP-43 and hnRNP C depletion may also relate to this, as well as differences in strength of depletion. Both TDP-43 and FUS proteins are known to bind their own mRNAs [68, 69] and so may compensate protein levels in response to shRNA knockdown.

Two genes, ATG4B and GPSM2, have previously been demonstrated to have cryptic exon inclusion RNA transcripts in ALS patient brain samples, suggesting a role for cryptic splicing in disease [25]. Our analysis also identified a cryptic exon in ATG4B in human cells, but not GPSM2; however we did not analyse human brain data. By expanding the list of cryptic exons, it will be interesting to explore whether these are also dysregulated in ALS patient brains. However, such analysis may prove challenging owing to the likely small concentrations of RNA originating from diseased cells in brain homogenate and the likelihood of degradation by NMD. Alternate strategies may involve mass spectrometry screens for the subset of cryptic exon containing genes that escape the NMD process and are translated into functional or truncated proteins. Such proteins may represent useful biomarkers for TDP-43 mislocalization and therefore ALS pathology.

A recent paper has used a complementary bioinformatic method to increase the number of cryptic exons seen in the Ling data [70]. This study extends the cryptic splicing phenomenon to RBM17, another RNA-binding protein. This finding makes the very low number of cryptic exons observed in the FUS depletion datasets even more surprising,

Conclusions

We confirm the presence of cryptic exons after TDP-43 depletion and show they have a negative impact on the genes they reside in, leading to decreased expression levels. Further work is warranted to determine the relevance of cryptic exons to ALS and FTD pathogenesis.

References

  1. 1.

    Matera AG, Wang Z. A day in the life of the spliceosome. Nat Rev Mol Cell Biol. 2014;15(2):108–21.

  2. 2.

    Eng L, Coutinho G, Nahas S, Yeo G, Tanouye R, Babaei M, D ̈ork T, Burge C, Gatti RA. Nonclassical splicing mutations in the coding and noncoding regions of the ATM gene: maximum entropy estimates of splice junction strengths. Hum Mutat. 2004;23(1):67–76.

  3. 3.

    Buratti E, Chivers M, Kralovicova J, Romano M, Baralle M, Krainer AR, Vorechovsky I. Aberrant 5′ splice sites in human disease genes: mutation pattern, nucleotide structure and comparison of computational tools that predict their utilization. Nucleic Acids Res. 2007;35(13):4250–63.

  4. 4.

    Vorechovsky I. Aberrant 3′ splice sites in human disease genes: mutation pattern, nucleotide structure and comparison of computational tools that predict their utilization. Nucleic Acids Res. 2006;34(16):4630–41.

  5. 5.

    Meili D, Kralovicova J, Zagalak J, Bonafe L, Fiori L, Blau N, Thony B, Vorechovsky I. Disease-causing mutations improving the branch site and polypyrimidine tract: Pseudoexon activation of LINE-2 and antisense alu lacking the poly(t)-tail. Hum Mutat. 2009;30(5):823–31.

  6. 6.

    Lewis BP, Green RE, Brenner SE. Evidence for the widespread coupling of alternative splicing and nonsense-mediated mRNA decay in humans. Proc Natl Acad Sci U S A. 2003;100(1):189–92.

  7. 7.

    McGlincy NJ, Smith CWJ. Alternative splicing resulting in nonsense-mediated mRNA decay: what is the meaning of nonsense? Trends Biochem Sci. 2008;33(8):385–93.

  8. 8.

    Deininger P, Prescott D. Alu elements: know the SINEs. Genome Biol. 2011;12(12):236.

  9. 9.

    Sorek R, Ast G, Graur D. Alu-containing exons are alternatively spliced. Genome Res. 2002;12(7):1060–7.

  10. 10.

    Vorechovsky I. Transposable elements in disease-associated cryptic exons. Hum Genet. 2010;127(2):135–54.

  11. 11.

    DeBoever C, Ghia EM, Shepard PJ, Rassenti L, Barrett CL, Jepsen K, Jamieson CHM, Carson D, Kipps TJ, Frazer KA. Transcriptome Sequencing Reveals Potential Mechanism of Cryptic 3′ Splice Site Selection in SF3B1-mutated Cancers. PLoS Comput Biol. 2015;11(3):1–19.

  12. 12.

    Zarnack K, K ̈onig J, Tajnik M, Martincorena In, Eustermann S, St’evant I, Reyes A, Anders S, Luscombe NM, Ule J. Direct competition between hnRNP C and U2AF65 protects the transcriptome from the exonization of alu elements. Cell. 2013;152(3):453–66.

  13. 13.

    Neumann M, Sampathu DM, Kwong LK, Truax AC, Micsenyi MC, Chou TT, Bruce J, Schuck T, Grossman M, Clark CM, McCluskey LF, Miller BL, Masliah E, Mackenzie IR, Feldman H, Feiden W, Kretzschmar HA, Trojanowski JQ, Lee VM-Y. Ubiquitinated TDP-43 in frontotemporal lobar degeneration and amyotrophic lateral sclerosis. Science. 2006;314(5796):130–3.

  14. 14.

    Sreedharan J, Blair IP, Tripathi VB, Hu X, Vance C, Rogelj B, Ackerley S, Durnall JC, Williams KL, Buratti E, Baralle F, de Belleroche J, Mitchell JD, Leigh PN, Al-Chalabi A, Miller CC, Nicholson G, Shaw CE. TDP-43 mutations in familial and sporadic amyotrophic lateral sclerosis. Science. 2008;319(5870):1668–72.

  15. 15.

    Vance C, Rogelj B, Hortob’agyi T, De Vos KJ, Nishimura AL, Sreedharan J, Hu X, Smith B, Ruddy D, Wright P, Ganesalingam J, Williams KL, Tripathi V, Al-Saraj S, Al-Chalabi A, Leigh PN, Blair IP, Nicholson G, de Belleroche J, Gallo J-M, Miller CC, Shaw CE. Mutations in FUS, an RNA processing protein, cause familial amyotrophic lateral sclerosis type 6. Science. 2009;323(5918):1208–11.

  16. 16.

    Buratti E, Baralle FE. Characterization and functional implications of the RNA binding properties of nuclear factor TDP-43, a novel splicing regulator of CFTR exon 9. J Biol Chem. 2001;276(39):36337–43.

  17. 17.

    Mercado PA, Ayala YM, Romano M, Buratti E, Baralle FE. Depletion of TDP 43 overrides the need for exonic and intronic splicing enhancers in the human apoA-II gene. Nucleic Acids Res. 2005;33(18):6000–10.

  18. 18.

    Bose JK, Wang I-F, Hung L, Tarn W-Y, Shen C-KJ. TDP-43 overexpression enhances exon 7 inclusion during the survival of motor neuron pre-mRNA splicing. J Biol Chem. 2008;283(43):28852–9.

  19. 19.

    Shiga A, Ishihara T, Miyashita A, Kuwabara M, Kato T, Watanabe N, Yamahira A, Kondo C, Yokoseki A, Takahashi M, Kuwano R, Kakita A, Nishizawa M, Takahashi H, Onodera O. Alteration of POLDIP3 splicing associated with loss of function of TDP-43 in tissues affected with ALS. PLoS One. 2012;7(8):43120.

  20. 20.

    Lagier-Tourenne C, Polymenidou M, Hutt KR, Vu AQ, Baughn M, Huelga SC, Clutario KM, Ling S-C, Liang TY, Mazur C, Wancewicz E, Kim AS, Watt A, Freier S, Hicks GG, Donohue JP, Shiue L, Bennett CF, Ravits J, Cleveland DW, Yeo GW. Divergent roles of ALS-linked proteins FUS/TLS and TDP-43 intersect in processing long pre-mRNAs. Nat Neurosci. 2012;15(11):1488–97.

  21. 21.

    Chiang P-M, Ling J, Jeong YH, Price DL, Aja SM, Wong PC. Deletion of TDP-43 down-regulates tbc1d1, a gene linked to obesity, and alters body fat metabolism. Proc Natl Acad Sci U S A. 2010;107(37):16320–4.

  22. 22.

    Shan X, PM C, Price DL, Wong PC. Altered distributions of gemini of coiled bodies and mitochondria in motor neurons of TDP-43 transgenic mice. Proc Natl Acad Sci. 2010;107(37):16325–30.

  23. 23.

    Polymenidou M, Lagier-Tourenne C, Hutt KR, Huelga SC, Moran J, Liang TY, Ling S-C, Sun E, Wancewicz E, Mazur C, Kordasiewicz H, Sedaghat Y, Donohue JP, Shiue L, Bennett CF, Yeo GW, Cleveland DW. Long pre-mRNA depletion and RNA missplicing contribute to neuronal vulnerability from loss of TDP-43. Nat Neurosci. 2011;14(4):459–68.

  24. 24.

    Arnold ES, SC L, Huelga SC, Lagier-Tourenne C, Polymenidou M, Ditsworth D, Kordasiewicz HB, McAlonis-Downes M, Platoshyn O, Parone PA, Da Cruz S, Clutario KM, Swing D, Tessarollo L, Marsala M, Shaw CE, Yeo GW, Cleveland DW. ALS-linked TDP-43 mutations produce aberrant RNA splicing and adult-onset motor neuron disease without aggregation or loss of nuclear TDP-43. Proc Natl Acad Sci. 2013;110(8):736–45.

  25. 25.

    Ling JP, Pletnikova O, Troncoso JC, Wong PC. TDP-43 repression of nonconserved cryptic exons is compromised in ALS-FTD. Science. 2015;349(6248):650–5.

  26. 26.

    Dobin A, Davis CA, Schlesinger F, Drenkow J, Zaleski C, Jha S, Batut P, Chaisson M, Gingeras TR. STAR: ultrafast universal RNA-seq aligner. Bioinformatics. 2013;29(1):15–21.

  27. 27.

    Tollervey JR, Curk T, Rogelj B, Briese M, Cereda M, Kayikci M, Konig J, Hortobagyi T, Nishimura AL, Zupunski V, Patani R, Chandran S, Rot G, Zupan B, Shaw CE, Ule J. Characterizing the RNA targets and position-dependent splicing regulation by TDP-43. Nat Neurosci. 2011;14(4):452–8.

  28. 28.

    Rogelj B, Easton LE, Bogu GK, Stanton LW, Rot G, Curk T, Zupan B, Sugimoto Y, Modic M, Haberman N, Tollervey J, Fujii R, Takumi T, Shaw CE, Ule J. Widespread binding of FUS along nascent RNA regulates alternative splicing in the brain. Sci Rep. 2012;2:603.

  29. 29.

    Van Nostrand EL, Pratt GA, Shishkin AA, Gelboin-Burkhart C, Fang MY, Sundararaman B, Blue SM, Nguyen TB, Surka C, Elkins K, Stanton R, Rigo F, Guttman M, Yeo GW. Robust transcriptome-wide discovery of RNA-binding protein binding sites with enhanced CLIP (eCLIP). Nat Methods. 2016;13(6):508–14.

  30. 30.

    Hartley SW, Mullikin JC. Detection and visualization of differential splicing in RNA-Seq data with JunctionSeq. Nucleic Acids Res. 2016;44(15):127. 1512.06038.

  31. 31.

    Li, YI, Knowles DA, Pritchard JK. LeafCutter: Annotation-free quantification of RNA splicing. bioRxiv. 2016;044107:1–31.

  32. 32.

    Vaquero-Garcia J, Barrera A, Gazzara MR, Gonz’alez-Vallinas J, Lahens NF, Hogenesch JB, Lynch KW, Barash Y. A new view of transcriptome complexity and regulation through the lens of local splicing variations. elife. 2016;5:1–30.

  33. 33.

    Goldstein LD, Cao Y, Pau G, Lawrence M, Wu TD, Seshagiri S, Gentleman R. Prediction and quantification of splice events from RNA-seq data. PLoS One. 2016;11(5):1–18.

  34. 34.

    Li H, Handsaker B, Wysoker A, Fennell T, Ruan J, Homer N, Marth G, Abecasis G, Durbin R. 1000 Genome Project Data Processing Subgroup: The sequence Alignment/Map format and SAMtools. Bioinformatics. 2009;25(16):2078–9.

  35. 35.

    Quinlan AR, Hall IM. BEDTools: a flexible suite of utilities for comparing genomic features. Bioinformatics. 2010;26(6):841–2.

  36. 36.

    Anders S, Reyes A, Huber W. Detecting differential usage of exons from RNA-seq data. Genome Res. 2012;22(10):2008–17.

  37. 37.

    Humphrey J, Plagnol V. Cryptex. https://github.com/jackhump/CryptEx. Accessed May 2017.

  38. 38.

    Ryan D. DEXSeq for intron retention. http://seqanswers.com/forums/archive/index.php/t-42420.html. Accessed Feb 2016.

  39. 39.

    Anders S, Pyl PT, Huber W. HTSeq–a python framework to work with high-throughput sequencing data. Bioinformatics. 2015;31(2):166–9.

  40. 40.

    Katz Y, Wang ET, Airoldi EM, Burge CB. Analysis and design of RNA sequencing experiments for identifying isoform regulation. Nat Methods. 2010;7(12):1009–15.

  41. 41.

    Bailey TL, Boden M, Buske FA, Frith M, Grant CE, Clementi L, Ren J, Li WW, Noble WS. MEME SUITE: tools for motif discovery and searching. Nucleic Acids Res. 2009;37(Web Server issue):202–8.

  42. 42.

    Heinz S, Sven H, Christopher B, Nathanael S, Eric B, Lin YC, Peter L, Cheng JX, Cornelis M, Harinder S, Glass CK. Simple combinations of Lineage-Determining transcription factors prime cis-regulatory elements required for macrophage and B cell identities. Mol Cell. 2010;38(4):576–89.

  43. 43.

    Crooks GE, Hon G, Chandonia JM, Brenner SE. WebLogo: a sequence logo generator. Genome Res. 2004;14(6):1188–90.

  44. 44.

    Smit AFA, Hubley R, Green P. RepeatMasker Open-4.0. 2015. http://www.repeatmasker.org. Accessed Feb 2016.

  45. 45.

    Pollard KS, Hubisz MJ, Rosenbloom KR, Siepel A. Detection of nonneutral substitution rates on mammalian phylogenies. Genome Res. 2010;20(1):110–21.

  46. 46.

    Love MI, Huber W, Anders S. Moderated estimation of fold change and dispersion for RNA-seq data with DESeq2. Genome Biol. 2014;15(12):550.

  47. 47.

    Yeo G, Gene Y, Burge CB. Maximum entropy modeling of short sequence motifs with applications to RNA splicing signals. J Comput Biol. 2004;11(2-3):377–94.

  48. 48.

    Wong JJL, Ritchie W, Ebner OA, Selbach M, Wong JWH, Huang Y, Gao D, Pinello N, Gonzalez M, Baidya K, Thoeng A, Khoo TL, Bailey CG, Holst J, Rasko JEJ. Orchestrated intron retention regulates normal granulocyte differentiation. Cell. 2013;154(3):583–95.

  49. 49.

    Braunschweig U, Barbosa-Morais NL, Pan Q, Nachman EN, Alipanahi B, Gonatopoulos-Pournatzis T, Frey B, Irimia M, Blencowe BJ. Widespread intron retention in mammals functionally tunes transcriptomes. Genome Res. 2014;24(11):1774–86.

  50. 50.

    Li Y, Rao X, Mattox WW, Amos CI, Liu B. RNA-Seq analysis of differential splice junction usage and intron retentions by DEXSeq. PLoS One. 2015;10(9):0136653.

  51. 51.

    Bai Y, Ji S, Wang Y. IRcall and IRclassifier: two methods for flexible detection of intron retention events from RNA-Seq data. BMC Genomics. 2015;16 Suppl 2:9.

  52. 52.

    Merkin J, Russell C, Chen P, Burge CB. Evolutionary dynamics of gene and isoform regulation in Mammalian tissues. Science. 2012;338(6114):1593–9.

  53. 53.

    Lonsdale J, Thomas J, Salvatore M, Phillips R, Lo E, Shad S, Hasz R, Walters G, Garcia F, Young N, Moore HF. The Genotype-Tissue Expression (GTEx) project. Nat Genet. 2013;45(6):580–5.

  54. 54.

    Huppertz I, Ina H, Jan A, Andrea D, Easton LE, Sibley CR, Yoichiro S, Mojca T, Julian K, Jernej U. iCLIP: Protein–RNA interactions at nucleotide resolution. Methods. 2014;65(3):274–87.

  55. 55.

    Kelley DR, Hendrickson DG, Tenen D, Rinn JL. Transposable elements modulate human RNA abundance and splicing via specific RNA-protein interactions. Genome Biol. 2014;15(12):537.

  56. 56.

    Blokhuis AM, Koppers M, Groen EJN, van den Heuvel DMA, Dini Modigliani S, Anink JJ, Fumoto K, van Diggelen F, Snelting A, Sodaar P, Verheijen BM, Demmers JAA, Veldink JH, Aronica E, Bozzoni I, den Hertog J, van den Berg LH, Pasterkamp RJ. Comparative interactomics analysis of different ALS-associated proteins identifies converging molecular pathways. Acta Neuropathol. 2016;132(2):175–96.

  57. 57.

    Ling S-C, Albuquerque CP, Han JS, Lagier-Tourenne C, Tokunaga S, Zhou H, Cleveland DW. ALS-associated mutations in TDP-43 increase its stability and promote TDP-43 complexes with FUS/TLS. Proc Natl Acad Sci U S A. 2010;107(30):13318–23.

  58. 58.

    Freibaum BD, Chitta RK, High AA, Taylor JP. Global analysis of TDP-43 interacting proteins reveals strong association with RNA splicing and translation machinery. J Proteome Res. 2010;9(2):1104–20.

  59. 59.

    Mohagheghi F, Prudencio M, Stuani C, Cook C, Jansen-West K, Dickson DW, Petrucelli L, Buratti E. TDP-43 functions within a network of hnRNP proteins to inhibit the production of a truncated human SORT1 receptor. Hum Mol Genet. 2016;25(3):534–45.

  60. 60.

    Yap K, Lim ZQ, Khandelia P, Friedman B, Makeyev EV. Coordinated regulation of neuronal mRNA steady-state levels through developmentally controlled intron retention. Genes Dev. 2012;26(11):1209–23.

  61. 61.

    Mendell JT, Sharifi NA, Meyers JL, Martinez-Murillo F, Dietz HC. Nonsense surveillance regulates expression of diverse classes of mammalian transcripts and mutes genomic noise. Nat Genet. 2004;36(10):1073–8.

  62. 62.

    Yap K, Makeyev EV. Regulation of gene expression in mammalian nervous system through alternative pre-mRNA splicing coupled with RNA quality control mechanisms. Mol Cell Neurosci. 2013;56:420–8.

  63. 63.

    Stalekar M, Yin X, Rebolj K, Darovic S, Troakes C, Mayr M, Shaw CE, Rogelj B. Proteomic analyses reveal that loss of TDP-43 affects RNA processing and intracellular transport. Neuroscience. 2015;293:157–70.

  64. 64.

    Collins MA, An J, Hood BL, Conrads TP, Bowser RP. Label-Free LC-MS/MS proteomic analysis of cerebrospinal fluid identifies Protein/Pathway alterations and candidate biomarkers for amyotrophic lateral sclerosis. J Proteome Res. 2015;14(11):4486–501.

  65. 65.

    Ruggiu M, Herbst R, Kim N, Jevsek M, Fak JJ, Mann MA, Fischbach G, Burden SJ, Darnell RB. Rescuing Z agrin splicing in nova null mice restores synapse formation and unmasks a physiologic defect in motor neuron firing. Proc Natl Acad Sci. 2009;106(9):3513–8.

  66. 66.

    Gilks N, Kedersha N, Ayodele M, Shen L, Stoecklin G, Dember LM, Anderson P. Stress granule assembly is mediated by prion-like aggregation of tia-1. Mol Biol Cell. 2004;15(12):5383–98.

  67. 67.

    Attig J, De Los Mozos IR, Haberman N, Wang Z, Emmett W, Zarnack K, Koenig J, Ule J. Splicing repression allows the gradual emergence of new alu-exons in primate evolution. elife. 2016;5(NOVEMBER2016):1–27.

  68. 68.

    Koyama A, Sugai A, Kato T, Ishihara T, Shiga A, Toyoshima Y, Koyama M, Konno T, Hirokawa S, Yokoseki A, Nishizawa M, Kakita A, Takahashi H, Onodera O. Increased cytoplasmic TARDBP mRNA in affected spinal motor neurons in ALS caused by abnormal autoregulation of TDP-43. Nucleic Acids Res. 2016;499.

  69. 69.

    Zhou Y, Liu S, Liu G, Öztürk A, Hicks GG. ALS-Associated FUS Mutations Result in Compromised FUS Alternative Splicing and Autoregulation. PLoS Genet. 2013;9(10):e1003895.

  70. 70.

    Tan Q, Krishna Yalamanchili H, Park J, De Maio A, Lu H-C, Wan Y-W, White JJ, Bondar VV, Sayegh LS, Liu X, Gao Y, Sillitoe RV, Orr HT, Liu Z, Zoghbi HY. Extensive cryptic splicing upon loss of rbm17 and tdp43 in neurodegeneration models. Hum Mol Genet. 2016;25(23):5083–93.

  71. 71.

    Amaral PP, Clark MB, Gascoigne DK, Dinger ME, Mattick JS. lncrnadb: a reference database for long noncoding rnas. Nucleic Acids Res. 2011;39(1):146.

Download references

Acknowledgements

The authors would like to thank all members of the Plagnol, Pritchard, Fratta and Isaacs labs for their assistance and discussion. We are extremely grateful for the RNA-seq, iCLIP and eCLIP data made freely available by the Cleveland, Gravely, Wong, Ule and Yeo labs. We are also grateful to Yang Li and Jonathan Pritchard for generously providing the processed GTEx and mouse tissue junctions.

Funding

J.H. is supported by a Medical Research Council and Brain Research Trust PhD studentship. The work of W.E. is supported by the Wellcome Trust (103760/Z/14/Z) and the Francis Crick Institute, which receives its core funding from Cancer Research UK (FC001002), the UK Medical Research Council (FC001002), and the Wellcome Trust (FC001002). P.F. is funded by a Medical Research Council/Motor Neuron Disease Association LEW Fellowship and by the NIHR UCLH BRC. A.M.I. is funded by Alzheimers Research UK, the Motor Neuron Disease Association and the European Research Council.

Availability of data and materials

For data availability see Table 2. All software written for this paper is available at [37].

Authors’ contributions

JH and VP wrote all the code used to analyse the data with input from WE. JH, VP, PF, and AMI designed the experiments. JH wrote the manuscript with discussion and approval from all authors.

Competing interests

The authors declare that they have no competing interests.

Consent for publication

Not applicable.

Ethics approval and consent to participate

Not applicable.

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Author information

Affiliations

  1. University College London Genetics Institute, Gower Street, London, UK
    • Jack Humphrey
    • , Warren Emmett
    •  & Vincent Plagnol
  2. Department of Neurodegenerative Disease, UCL Institute of Neurology, Queen Square, London, UK
    • Jack Humphrey
    •  & Adrian M. Isaacs
  3. Department of Molecular Neuroscience, UCL Institute of Neurology, Queen Square, London, UK
    • Warren Emmett
  4. The Francis Crick Institute, Midland Road, London, UK
    • Warren Emmett
  5. Department of Motor Neuroscience and Movement Disorders, UCL Institute of Neurology, Queen Square, London, UK
    • Pietro Fratta
Authors
  1. Search for Jack Humphrey in:
  2. Search for Warren Emmett in:
  3. Search for Pietro Fratta in:
  4. Search for Adrian M. Isaacs in:
  5. Search for Vincent Plagnol in:

Corresponding author

Correspondence to Jack Humphrey.

Additional files

Additional file 1: Figure S1.

Pre-classification output of CryptEx pipeline demonstrates a variety of novel splicing events in TDP-43, FUS and hnRNP C depletion data. Every novel splicing event plotted by mean depth of reads covering the novel event against log2(fold change) between depletion and control samples. The cryptic exon classifier throws out any splicing event where the canonical intron in which the cryptic splicing event appears is represented by less than five spliced reads (purple) or where the |log2(fold change)| < 0.6 (light blue). Splicing events are classified as cryptic exons if the spliced reads agree with the rest of the reads and have at least 1 spliced read per sample (red). Those that fail this step are coloured orange. (ZIP 1386 kb)

Additional file 2: Figure S2.

Each cryptic exon discovered in either of the two mouse datasets. For each dataset, the biological replicates were combined to create merged BAM files for each condition. The BAM files were loaded into IGV for visualisation. Read coverage and splice junctions are shown. The Ensembl transcripts for the mm10 build are provided, as are the coordinates of the cryptic exons discovered by CryptEx. (PDF 2436 kb)

Additional file 3: Figure S3.

Each cryptic exon discovered in either of the two human K562 datasets. As above, with the hg38 human genome build. (PDF 5917 kb)

Additional file 4: Tables S1 and S2.

Quantification of all results for each cryptic exon discovered by CryptEx in mouse (ST1) and human (ST2). Change in percent spliced in (∆PSI) scores were calculated by taking the difference of ratios of novel splice junctions over the sum of novel and annotated (intron-spanning) splice junctions in control and depletion samples for the 5′ and 3′ splice junctions. (ZIP 8 kb)

Additional file 5: Tables S5 and S6.

Inclusion of cryptic exons in normal mouse (ST5) and human (ST6) tissues. RNA-seq data from multiple mouse tissues from [52] and multiple human tissues from the GTEx project [53] was downloaded from the Sequence Read Archive (accession PRJNA177791) and dbGap (phs000424.v6.p1) respectively. All samples were aligned with STAR using two-pass mapping. The resulting junction coordinates were grouped into overlapping clusters for each tissue using Leafcutter [31]. A custom R script then queried the resulting junction tables for evidence of junctions belonging to the previously discovered mouse and human cryptic exons, as well as the canonical junctions in which the cryptic exons splice to and from. The counts of upstream and downstream junctions in each sample were divided by the counts of the canonical junction to produce an inclusion ratio. For each cryptic exon that was detected, the mean inclusion ratio for each tissue is presented with the standard deviation. For the 52 mouse cryptic exons, only 4 showed any evidence of being included in normal tissues. Reep3 E001i1 and Adipor2 E010i2 are included in a few tissues at very low levels. Elmod1 E003i2 is seen in brain tissue at an inclusion rate above 10%, whereas Thoc7 E007i1 was included in every tissue bar heart. However, the inclusion rates were highly variable. Among the 95 human cryptic exons, only three were detected in 49 different human tissues from the GTEx project. MPDZ E015i1, UHRF2 E017i2 and DEAF1 E005i2 were all detected in at least 1 tissue. Only UHRF2 E017i2 was regularly seen above 10% inclusion, albeit with very high variance between samples. (PDF 66 kb)

Additional file 6: Figure S4.

Motif finding with HOMER The top ten motifs reported by the algorithm when comparing flanked cryptic exons with adjacent intronic sequence. The red asterisk indicates that the motif is potentially a false positive result. (TIF 1799 kb)

Additional file 7: Tables S3 and S4.

All repeat elements enriched in mouse (ST3) and human (ST4) cryptic exons. For each class of repeat element that was enriched in a set of cryptic exons, the exact overlapping repeat element was compiled into a table. The strand column refers to the orientation of the gene, not the repeat element. For the simple repeats, all annotations are made in the positive direction. Therefore (AC)n containing repeats in the antisense direction are in fact (GT)n repeats for genes on the negative strand. Figure S5. The RNA sequence of the B2 SINE in the antisense orientation. The DNA sequence of the B2 SINE was downloaded from lncrnadb [71] and converted to the reverse complement to get its antisense orientation. Ts were changed to Us to reflect the RNA sequence. Stretches of UG and GU are highlighted in red. (PDF 123 kb)

Rights and permissions

Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Humphrey, J., Emmett, W., Fratta, P. et al. Quantitative analysis of cryptic splicing associated with TDP-43 depletion. BMC Med Genomics 10, 38 (2017) doi:10.1186/s12920-017-0274-1

Download citation

Keywords

  • RNA-seq
  • Cryptic exons
  • Splicing
  • TDP-43

BMC Medical Genomics

ISSN: 1755-8794

Contact us