Purifying selection of long dsRNA is the first line of defense against false activation of innate immunity
Genome Biology volume 21, Article number: 26 (2020)
Mobile elements comprise a large fraction of metazoan genomes. Accumulation of mobile elements is bound to produce multiple putative double-stranded RNA (dsRNA) structures within the transcriptome. These endogenous dsRNA structures resemble viral RNA and may trigger false activation of the innate immune response, leading to severe damage to the host cell. Adenosine to inosine (A-to-I) RNA editing is a common post-transcriptional modification, abundant within repetitive elements of all metazoans. It was recently shown that a key function of A-to-I RNA editing by ADAR1 is to suppress the immunogenic response by endogenous dsRNAs.
Here, we analyze the transcriptomes of dozens of species across the Metazoa and identify a strong genomic selection against endogenous dsRNAs, resulting in their purification from the canonical transcriptome. This purifying selection is especially strong for long and nearly perfect dsRNAs. These are almost absent from mRNAs, but not pre-mRNAs, supporting the notion of selection due to cytoplasmic processes. The few long and nearly perfect structures found in human transcripts are weakly expressed and often heavily edited.
Purifying selection of long dsRNA is an important defense mechanism against false activation of innate immunity. This newly identified principle governs the integration of mobile elements into the genome, a major driving force of genome evolution. Furthermore, we find that most ADAR1 activity is not required to prevent an immune response to endogenous dsRNAs. The critical targets of ADAR1 editing are, likely, to be found mostly in non-canonical transcripts.
Most invading viruses give rise to long double-stranded RNAs (dsRNAs) in the cytoplasm of the host cells . These structures are identified by sensor proteins such as MDA5 and trigger the production of type I interferons as part of recruiting the innate immunity system [2, 3]. However, large numbers of endogenous dsRNAs are likely to appear in normal eukaryotic cells as well , mainly due to the abundance of mobile elements in the genome—transcripts harboring nearby inverted copies of the same repeat fold to create an endogenous dsRNA structure . Therefore, distinguishing between self and non-self dsRNAs is critical for proper innate immune activity.
It was pointed out recently that the main function of the essential ADAR1 enzyme, conferring adenosine to inosine (A-to-I) RNA editing, is to prevent activation of cytosolic immune response [6,7,8,9,10]. A-to-I editing, mostly carried out by the constitutive ADAR1p110 variant, introduces mismatches to the endogenous dsRNAs while still in the nucleus [11, 12], so that the edited endogenous transcripts are no longer recognized by dsRNA sensors in the cytoplasm. As mobile element activity goes on, more and more putative dsRNAs accumulate in the transcriptome, and the burden on ADAR1, constitutively marking all of these targets to prevent false activation of innate immunity, becomes increasingly heavier. Therefore, one may hypothesize that even in the presence of ADAR1 editing, endogenous dsRNAs have a detrimental effect and should be selected against. Such selection would then have an impact on the proliferation of repetitive elements in the DNA, a major driving force for genome evolution .
Furthermore, editing levels are usually quite low within paired inverted Alu repeats, the archetypal examples of human endogenous dsRNAs [14,15,16,17]. Although many adenosines are editable in each Alu repeat, most of these are converted into inosine only in < 1% of the transcripts . Accordingly, the average number of inosines per double-stranded region in an RNA molecule is often lower than one, at least for the less-edited tissues, and the majority of individual molecules are not edited at all . Thus, it seems that editing cannot fully protect from false activation of innate immunity by these endogenous dsRNAs, or else that the typical editing target does not pose a risk of such false activation, edited or unedited.
Here, we study the repertoire of putative dsRNA structures in mRNA and pre-mRNA molecules. We analyze the transcriptomes of 49 organisms, from yeast to human, and find that dsRNAs in mRNA molecules are strongly depleted from the genome. This demonstrates a strong selective force that controls the integration of repetitive elements into genes in order to minimize the number of endogenous dsRNAs. Notably, in pre-mRNA molecules (including the introns), such depletion is much weaker. This indicates that the main driving forces of this selection process are cytoplasmic, presumably the need to avoid activation of innate immunity sensors by endogenous RNA. Moreover, long and nearly perfect RNA duplexes, reported to be the prime targets of MDA5 [19, 20], are strongly depleted even in pre-mRNA or expressed at a low level leading to a weaker selective pressure. Finally, we find that some of the few long and nearly perfect dsRNAs that are not purified from the human genome undergo heavy RNA editing. Such loci may be critical ADAR1 targets.
In order to explore the extent to which mature RNA molecules and pre-mRNA molecules form long and stable dsRNA structures, we employ a cross-species whole transcriptome approach, studying the full transcriptome of 49 organisms included in the Ensembl database , from yeast to human (Additional file 1: Table S1). Altogether, we analyzed pre-mRNA (genomic sequence from the beginning of the first exon to the end of the last exon, including introns) and the much shorter mature RNA sequences for 724,071 different genes (14,777 per organism, on average), covering 21.7 Gbp.
Despite important recent technological advancements, predicting the detailed structure of RNA molecules, including structural motifs, protein-binding regions, and RNA-RNA interactions, is yet a major challenge. Numerous computational tools are available for predicting RNA secondary structures, but their reliability in predicting full-length molecule structure is limited . Thus, full understanding of the RNA folds requires intricate experimental approaches, currently inapplicable at large scale . However, here, we are not interested in the full and accurate structure, but rather focus on long dsRNA stems, > 40 bp long. These substructures are easily detected by standard sequence alignment tools, e.g., BLAST —if a long region of a molecule is highly similar to the reverse complement of another region in the same molecule, these two regions are likely to pair together and form a long and stable dsRNA. We thus use BLAST to align each of the mRNA and the pre-mRNA sequences to itself, and count the number of reversely oriented duplicated sequences (inverted duplicated sequences, IDS) as well as the total number of nucleotides involved. BLAST is not a perfect predictor of dsRNA stems, as it does not take into account the different pairing energies of A:T and G:C pairs and ignores the binding energy of G:U pairs. However, the size of the database we searched prevents using the much slower RNA folding algorithms, and for long and nearly perfect stems, BLAST provides a reasonable approximation. As a natural control, we look at the number of same-strand hits, showing similar sequence identity for regions on the same strand (tandem duplicated sequences, TDS), which are not relevant to the secondary double-stranded structure (Fig. 1).
One immediately notices a global depletion of IDSs in mRNA molecules, compared to the control TDSs (see Fig. 2). Looking at all organisms combined, one finds only 6525 IDSs in mRNAs covering 786 kbp, compared with 42,946 TDSs covering 3.01 Mbp (p < 1e−100; see Additional file 1: Table S2). This depletion indicates a strong selection against long and stable duplexes in the mRNA, consistent across most organisms. Furthermore, the selection against dsRNAs is much weaker in the pre-mRNA, suggesting it is driven by cytoplasmic processes (57.5M IDSs covering 1.26 Gbp, compared with 61.3M TDSs covering 1.51 Gbp; p < 1e−100). Limiting the gap between the 2 duplicated sequences to 2000 bp does not change the results, qualitatively (Additional file 2: Figure S1). This is consistent with the notion of avoidance of innate immunity activation by endogenous RNA, as viral dsRNA sensors are active in the cytoplasm . Note, however, that stronger depletion of dsRNAs in pre-mRNAs is observed in a few species. For example, yeast introns are uncommon , and thus, the pre-mRNA is almost identical to the mRNA. Similarly, while honeybees do have an ADAR enzyme , very few retroelements have been identified in the honeybee genome , which could account for the lower number of dsRNAs in introns.
Long and nearly perfect duplexes are the prime candidates to provoke an innate immune response, as they resemble viral dsRNAs [25, 29]. Consistently, we observe a stronger genomic depletion for longer and highly base-paired structures (Fig. 3 and Additional file 2: Figure S2). There are only 246 almost perfectly base-paired IDSs (putative helices with > 96% identity), compared with 3436 almost perfect TDSs (32,245 bp vs. 425,753 bp) in all organisms (p < 1e−100). Moreover, depletion of almost perfect hits is noticeable even for pre-mRNAs (1.07M TDSs vs. 0.78M IDSs (p < 1e−100); 205 Mbp vs. 81 Mbp, respectively; Additional file 2: Figure S2 and Additional file 1: Table S3). Similarly, strong depletion is observed for long (> 300 bp) IDSs in mRNAs, with only 195 structures covering 91,310 bp, compared with 3915 TDSs covering 1.41 Mbp (p < 1e−100). In pre-mRNA molecules, one finds only 1.57M long IDSs compared with 2.31M long TDSs (p < 1e−100; 401 Mbp vs. 608 Mbp, respectively) (Additional file 2: Figure S2 and Additional file 1: Table S4). Finally, IDSs that are both long and almost perfectly matching are extremely rare, only 4 such examples are present in mRNA sequences of all organisms examined (manual inspection suggests these are unreliable), compared with 258 such TDSs (p = 2.6e−71; 54,479 vs. 144,989 structures in pre-mRNA) (Fig. 3 and Additional file 1: Table S5). We conclude that long and nearly perfect dsRNA structures are almost nonexistent in mature RNAs and selected against even if they are present only in the pre-mRNA molecules. A possible explanation for the depletion in pre-mRNA is that regions annotated as introns might actually be mis-annotated exons (constitutive or alternative), especially in less-explored transcriptomes. In addition, there might be a selective pressure even against intronic dsRNAs due to the occasional intron retention as a result of imperfect splicing. Although rare, dsRNAs present in these aberrantly spliced transcripts may trigger the immune system and therefore are selected against.
To further support the idea that depletion of IDSs within transcripts is related to the potential risk of endogenous dsRNAs, we study the expression level of all IDSs identified within RefSeq human transcripts in a pool of 30 RNA-seq GTEx  samples, originating from 15 different tissues (Additional file 1: Table S6). We find that the expression of IDSs negatively correlates with their length and identity (Fig. 4a, b), as expected if the driving selective disadvantage relates to the expressed RNA molecules. To exclude the possibility of reverse-transcription artifacts related to the secondary structures, we verified that the regions that show no expression in mRNA-seq data are actually well-covered in total RNA datasets, suggesting that the reverse transcription does allow their amplification (Additional file 2: Figure S3). Note that expression here refers to that of the IDS region, which could be much lower than the expression level of the hosting gene, as the IDS is mostly due to intronic sequences.
The above results suggest that the main suppressor of innate immune response that may be triggered by endogenous double-stranded RNAs is a tight purifying genomic selection. However, the balance between the continuous introduction of new putative dsRNAs, mainly due to the proliferation of repetitive elements, and the pruning of dangerous dsRNAs by purifying selection may lead to a residual number of potentially dangerous structures. In fact, we do see that most dsRNA structures reside in repetitive sequences (counting unique dsRNA genomic nucleotides overlapping known repeats: 531/786 kbp in mRNAs and 707/1260 Mbp in pre-mRNAs, for organisms with repetitive elements annotation; Additional file 1: Table S7). Furthermore, the depletion of IDSs in mRNA (but not pre-mRNA) is stronger for dsRNAs not associated with repetitive elements (Additional file 2: Figure S4). These observations are consistent with the view that dsRNAs associated with repetitive elements are being continuously added to the genome, and the purifying selection against them is still ongoing, maintaining the number of long and nearly perfect self-dsRNAs under control.
It was suggested recently that editing by ADAR1 plays an important role in preventing the activation of cytosolic response [7,8,9,10]. Using the abovementioned pool of GTEx tissues, we studied the editing levels in all 197 human IDSs within RefSeq transcripts that are both longer than 300 bp and with identity above 96% (Additional file 1: Table S8). Of these, in only 20 (10%), both arms of the IDSs are expressed at a level exceeding FPKM = 0.01 (to give perspective, FPKM = 1 corresponds, roughly , to 0.2–2 RNA molecules per cell). Seven of these are indeed edited strongly enough to bring the edited structure below the 96% identity cutoff (Fig. 4c). Only 2 IDSs are expressed at levels exceeding FPKM = 0.1, and both become much less base-paired by editing (one of these is presented in detail in Fig. 4d). Looking at another pool of 30 samples from the weakly edited muscle tissue (Additional file 1: Table S6), only 12 IDSs (6%) pass the FPKM = 0.01 cutoff, and in 5 of them, editing brings the identity below 96%. Not a single IDS is expressed stronger than FPKM = 0.1 in this pool (Additional file 1: Table S8).
We thus find that purifying genomic selection is the main contributor to protection against false activation of a cytosolic response to canonical endogenous transcripts appearing in a reference transcriptome, such as RefSeq. To the extent ADAR1 editing has any role in this protection, it is limited to a handful of putative dsRNA structures. Clearly, the vast majority of ADAR1 editing activity is irrelevant for this protective role. Furthermore, many of the essential targets of ADAR1 reside, likely, out of canonical transcripts.
Most viral infections lead to long viral dsRNAs in the cytoplasm . These are recognized by the innate immunity sensors  and trigger a response involving activation of hundreds of genes, mainly through interferon type I pathways . Other dsRNA-based antiviral defense mechanisms are observed in organisms lacking the interferon pathway, such as the siRNA pathway in insects . This response to viral infections comes at a price of severe damage to the hosting cell and its surroundings and may even affect the entire organism. Therefore, it is crucial to prevent the misidentification of endogenous dsRNAs as a viral infection that would trigger the above response unnecessarily .
Throughout the course of evolution, organisms are bound to accumulate more and more new dsRNA structures. Most endogenous long and stable dsRNA structures are due to intra-molecular folding, rather than binding of two (possibly anti-sense) transcripts . Genomes are continuously bombarded by mobile elements that are often integrated into the genomic sequence. In many cases, the appearance of an active new element results in a dramatic accumulation of numerous nearly identical copies of the same element over a short period of time. These provide a natural source of new dsRNA structures—two reversely oriented copies of the same mobile elements introduced into a transcribed region of the DNA will be transcribed into the RNA molecule and form a long and nearly perfect dsRNA structure . The results presented here show how this influx of novel putative dsRNAs into the transcriptome is encountered by a global purifying selection.
Purifying selection is a major driving force of evolution, weeding out of the genome harmful alleles. Here, we demonstrated a general evolutionary principle that provides a fundamental layer of defense against false triggering of the viral infection response: Endogenous dsRNA-forming sequences that pose a risk of self-intolerance leading to cell death are either rooted out of the genome or silenced transcriptionally.
What is then the critical role of ADAR1 editing? As mobile element activity goes on, more and more repeats integrate into the transcribed part of the genome, and putative dsRNAs accumulate in the transcriptome . Some of these newly added sequences may pose a risk of undesired immune response. In the long run, these structures are likely to be eliminated from the genome through purifying selection, possibly even before they are fixated in the whole population. However, the balance between these two counteracting processes is bound to lead to a residual number of somatic or polymorphic potentially dangerous transcripts. Alternatively, such offending structures may appear in lowly expressed alternatively spliced exons or rarely expressed long 3′ UTRs. We hypothesize that handling these few targets is the raison d’etre of ADAR1 editing activity.
Strong depletion is observed for long and nearly perfect dsRNAs, consistent with previous studies of MDA5/MAVS specificity. However, short (< 300 bp) and imperfect (identity < 96%) dsRNAs are also purified from mRNAs. Why would these be depleted? Possibly, even shorter and imperfect RNA duplexes may be recognized by dsRNA sensors to some extent. Alternatively, an overload of ADAR1-binding transcripts might have a detrimental effect on ADAR1 protection, even if these transcripts themselves do not pose a risk. In addition, endogenous dsRNAs might have additional detrimental effects on RNA processing and translation [36,37,38,39].
Integration of mobile elements is one of the major mechanisms for genomic innovations . To date, not much is known of the rules governing these integration events. One of the few observations regarding mobile element fixation relates to a bias for same-strand orientation of neighboring elements due to recombination, specifically demonstrated for the primate-specific Alu element [41,42,43]. However, the depletion of dsRNAs found here is much stronger and specific to the expressed mRNA sequences. It even varies between mature RNAs and pre-mRNA regions. Thus, the selective force demonstrated here is essentially different in that it is governed by the RNA, and not the DNA, structure. Specifically, it is determined by distances on the mature RNA molecule, irrespective of the physical distance along the chromosome. The selective effect described here is therefore a new important rule shaping genome structure and evolution.
Finally, we would like to note that most of ADAR1 editing is not at all required for preventing the innate immune response. For example, most editing events in human exons occur due to exon-intron pairing. These exonic Alu elements do not have any complementary Alu sequence in the hosting mRNA sequence after splicing and thus do not pose any threat of dsRNA formation at the mRNA level. Moreover, these are typically edited in about one adenosine per Alu sequence , which is usually unlikely to confer major changes in the secondary structure. In addition, the majority of ADAR activity occurs in intron-intron pairs and modifies RNA sequences that are not transported to the cytoplasm at all. Thus, the fraction of ADAR1 activity that takes care of the rare endogenous dsRNA structures in mature RNA that poses a threat of misidentification by the innate immunity system is astonishingly minute. This testifies to the critical importance of handling these rare, recently introduced, dsRNAs that have yet evaded the genomic selection mechanism.
Ensemble  transcriptomes were downloaded from the UCSC site  for all 53 available organisms from different clades. We excluded 3 organisms for which < 200 genes were reported, as well as 1 case where there was an inconsistency between the mRNA and pre-mRNA data (Additional file 1: Table S1). Pre-mRNA transcripts longer than 1 million bp were discarded. Overlapping transcripts were removed, keeping only the longer variant for each gene. Genes with several genomic duplications were included only once. Genes mapped to mitochondria, haplotypes of standard chromosomes, and random or unknown chromosomes of the hg19 assembly were discarded. The organisms in our set are not all equally explored, leading to large variations in the reliability and coverage of the annotated transcriptomes. To partially mitigate this, we kept only protein-coding genes, which are better characterized. These filters resulted in 724,809 genes, 1 transcript per gene, with a total pre-mRNA length of 1.37 Gbp.
Quantifying the load of putative dsRNAs
For each gene, we used BLAST  to look for alignments of the sequence to itself, for both the pre-mRNA and the mRNA sequences, keeping only matches with length > 40 and identity > 70%. BLAST matches involving the two strands (plus/minus hits) are considered putative dsRNAs, while same-strand hits (plus/plus) are used as a control (Fig. 1b).
Often, the same region appears in multiple hits. We thus created a bed file from all reversely oriented or same-strand hits in an organism (within a given range of identity and length), merged the regions using bedtools sort and merge, and summed the number of genomic nucleotides in the merged regions. A nucleotide belonging to several hits was assigned to the longer of them.
Expression and editing in human tissues
We compiled a pool of 30 GTEx RNA-seq samples originating from 15 different human tissues (2 samples each) and another pool of GTEx muscle samples (representing a lowly edited tissue) (see Additional file 1: Table S6). Duplicated reads were removed using PRINSEQ lite (http://prinseq.sourceforge.net/index.html). RNA-seq data were aligned (as single-end reads) to the genome (hg19) using BWA  with default parameters. To account for heavily edited reads, reads that failed to align were re-aligned using the hyper-editing 3-letter approach , with default parameters. Some of the studied dsRNA regions are composed of 2 nearly identical regions. Thus, in addition to the uniquely aligned reads, we also included reads that were mapped to both arms of the putative dsRNA region and in an opposite orientation (they were assigned to one of the arms, randomly). Altogether, 1.343 billion (single-end) reads were mapped for the pool of 15 tissues and 1.419 billion for the muscle samples. In both cases, more than 99.9% of these were uniquely mapped by BWA.
Following alignment, we trimmed 5 bases from both ends of the read using trimBam of BamUtil . We then ran samtools mpileup  to find the number of reads matching the genomic A and the number of A-to-G mismatches, for each genomic adenosine within putative dsRNA regions. The sum of these 2 is the coverage of the genomic nucleotide, and the ratio of mismatches to coverage is its editing level. For each arm of the putative dsRNA, we define the coverage as the average coverage over all the adenosines within, and the editing index [12, 49] as the ratio of all A-to-G mismatches mapped to the region to the sum over the coverage of all adenosines. FPKM values were calculated based on the total number of reads used and their effective length following trimming. For example, 1.343 billion reads in the 15 tissue pool, with an effective length of 66 bp (after trimming 5 bp from each end of the 76-bp reads), translate to 1 FPKM = 88.64 coverage. We also calculate the average number of inosines per dsRNA structure (index times the number of adenosines). To estimate the contribution of editing to destabilization of the dsRNA structure, we define the residual identity between the arms as the original identity between the genomic sequences minus the ratio of average inosine number to region length (average length of both arms). This assumes that all inosines lead to destabilization, which is approximately correct for the tightly bound structures of interest here. For this analysis, we considered only dsRNA regions where both arms reside within the same RefSeq transcript. Overlapping dsRNA regions were discarded for this calculation, retaining only the one with the highest identity.
In order to exclude the possibility of no coverage due to technical reverse-transcription problems, we analyzed the expression level in the same regions for a dataset of total RNA-seq from 22 healthy human mammary tissues (GSE103001 ). We used the expression of a list of housekeeping exons  to normalize the expression FPKM values across mRNA and total RNA samples.
To calculate the fraction of paired regions belonging to genomic repeats, we used RepeatMasker annotation as downloaded taken from UCSC (when available). Tetraodon was excluded from this analysis, as there was no RepeatMasker annotation for this organism.
To test for significance of the disparity between numbers of IDS and TDS, we look at the observed fraction of IDSs among all duplicated sequences found, i.e., #IDS/(#IDS+#TDS), and use a single proportion test to reject the null hypothesis that IDS and TDS are equally probable (i.e., the fraction is 0.5 for the parent distribution).
Availability of data and materials
All sequencing data used in this study are publicly available. RNA-seq reads for this analysis were obtained from GTEx (see “Methods” section and Additional file 1: Table S6 for the list of RNA-seq files used). Ensembl transcriptomes were downloaded from the UCSC genome browser site (see the “Methods” section).
Weber F, Wagner V, Rasmussen SB, Hartmann R, Paludan SR. Double-stranded RNA is produced by positive-strand RNA viruses and DNA viruses but not in detectable amounts by negative-strand RNA viruses. J Virol. 2006;80:5059–64 [cited 2018 Feb 28]. Available from: http://jvi.asm.org/cgi/doi/10.1128/JVI.80.10.5059-5064.2006.
Wu J, Chen ZJ. Innate immune sensing and signaling of cytosolic nucleic acids. Annu Rev Immunol. 2014;32:461–88 [cited 2016 Jul 3]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/24655297.
Schneider WM, Chevillotte MD, Rice CM. Interferon-stimulated genes: a complex web of host defenses. Annu Rev Immunol. 2014;32:513–45.
Reich DP, Bass BL. Mapping the dsRNA world. Cold Spring Harb Perspect Biol. 2019;11:a035352 [cited 2019 Mar 12]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/30824577.
Porath HT, Knisbacher BA, Eisenberg E, Levanon EY. Massive A-to-I RNA editing is common across the Metazoa and correlates with dsRNA abundance. Genome Biol. 2017;18:185 [cited 2018 Oct 4]. Available from: http://genomebiology.biomedcentral.com/articles/10.1186/s13059-017-1315-y.
Hartner JC, Walkley CR, Lu J, Orkin SH. ADAR1 is essential for the maintenance of hematopoiesis and suppression of interferon signaling. Nat Immunol. 2009;10:109–15 Available from: http://www.ncbi.nlm.nih.gov/pubmed/19060901%0A. http://www.pubmedcentral.nih.gov/articlerender.fcgi?artid=PMC2701568.
Mannion NM, Greenwood SM, Young R, Cox S, Brindle J, Read D, et al. The RNA-editing enzyme ADAR1 controls innate immune responses to RNA. Cell Rep. 2014;9:1482–94 Elsevier. [cited 2016 Jul 13]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/25456137.
Liddicoat BJ, Piskol R, Chalk AM, Ramaswami G, Higuchi M, Hartner JC, et al. RNA editing by ADAR1 prevents MDA5 sensing of endogenous dsRNA as nonself. Science (80- ). 2015;349:1–9 [cited 2015 Jul 24]. Available from: http://www.sciencemag.org/cgi/doi/10.1126/science.aac7049.
Pestal K, Funk CC, Snyder JM, Price ND, Treuting PM, Stetson DB. Isoforms of RNA-editing enzyme ADAR1 independently control nucleic acid sensor MDA5-driven autoimmunity and multi-organ development. Immunity. 2015;43:933–44 [cited 2015 Nov 19]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/26588779.
George CX, Ramaswami G, Li JB, Samuel CE. Editing of cellular self-RNAs by adenosine deaminase ADAR1 suppresses innate immune stress responses. J Biol Chem. 2016;291:6158–68 [cited 2018 Mar 8]. Available from: http://www.jbc.org/lookup/doi/10.1074/jbc.M115.709014.
Patterson JB, Samuel CE. Expression and regulation by interferon of a double-stranded- RNA-specific adenosine deaminase from human cells: evidence for two forms of the deaminase. 1995;15:5376–88 Available from: http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?cmd=Retrieve&db=PubMed&dopt=Citation&list_uids=7565688.
Roth SH, Levanon EY, Eisenberg E. Genome-wide quantification of ADAR adenosine-to-inosine RNA editing activity. Nat Methods. 2019;16:1131–8 [cited 2019 Nov 5]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/31636457.
Cordaux R, Batzer MA. The impact of retrotransposons on human genome evolution. Nat Rev Genet. 2009;10:691–703 Nature Publishing Group;[cited 2014 Jul 11]. Available from: http://www.pubmedcentral.nih.gov/articlerender.fcgi?artid=2884099&tool=pmcentrez&rendertype=abstract.
Levanon EY, Eisenberg E, Yelin R, Nemzer S, Hallegger M, Shemesh R, et al. Systematic identification of abundant A-to-I editing sites in the human transcriptome. Nat Biotechnol. 2004;22:1001–5 Available from: http://www.nature.com/nbt/journal/v22/n8/full/nbt996.html%5Cn. http://www.nature.com/nbt/journal/v22/n8/pdf/nbt996.pdf.
Blow M, Futreal AP, Wooster R, Stratton MR. A survey of RNA editing in human brain. Genome Res. 2004;14:2379–87 Available from: http://www.ncbi.nlm.nih.gov/pubmed/15545495.
Kim DDY, Kim TTY, Walsh T, Kobayashi Y, Matise TC, Buyske S, et al. Widespread RNA editing of embedded Alu elements in the human transcriptome. Genome Res. 2004;14:1719–25 Available from: http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?cmd=Retrieve&db=PubMed&dopt=Citation&list_uids=15342557.
Athanasiadis A, Rich A, Maas S. Widespread A-to-I RNA editing of Alu-containing mRNAs in the human transcriptome. PLoS Biol. 2004;2:e391 Available from: http://www.ncbi.nlm.nih.gov/pubmed/15534692.
Bazak L, Haviv A, Barak M, Jacob-Hirsch J, Deng P, Zhang R, et al. A-to-I RNA editing occurs at over a hundred million genomic sites, located in a majority of human genes. Genome Res. 2014;24:365–76 [cited 2013 Dec 18]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/24347612.
Wu B, Peisley A, Richards C, Yao H, Zeng X, Lin C, et al. Structural basis for dsRNA recognition, filament formation, and antiviral signal activation by MDA5. Cell. 2013;152:276–89 [cited 2019 Apr 29]. Available from: https://linkinghub.elsevier.com/retrieve/pii/S0092867412014365.
Peisley A, Lin C, Wu B, Orme-Johnson M, Liu M, Walz T, et al. Cooperative assembly and dynamic disassembly of MDA5 filaments for viral dsRNA recognition. Proc Natl Acad Sci U S A. 2011;108:21010–5 [cited 2019 Nov 7]. Available from: http://www.pnas.org/cgi/doi/10.1073/pnas.1113651108.
Flicek P, Amode MR, Barrell D, Beal K, Billis K, Brent S, et al. Ensembl 2014. Nucleic Acids Res. 2014;42:D749–55 [cited 2016 Jul 4]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/24316576.
Cruz JA, Westhof E. The dynamic landscapes of RNA architecture. 2009;136:604–9 [cited 2019 Apr 29]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/19239882.
Bevilacqua PC, Ritchey LE, Su Z, Assmann SM. Genome-wide analysis of RNA secondary structure. Annu Rev Genet. 2016;50:235–66 [cited 2019 Apr 29]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/27648642.
Altschul SF, Gish W, Miller W, Myers EW, Lipman DJ. Basic local alignment search tool. J Mol Biol. 1990;215:403–10 [cited 2016 Oct 13]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/2231712.
Dias Junior AG, Sampaio NG, Rehwinkel J. A balancing act: MDA5 in antiviral immunity and autoinflammation. Trends Microbiol. 2019;27:75–85 [cited 2019 Apr 15]. Available from: https://linkinghub.elsevier.com/retrieve/pii/S0966842X18301793.
Neuvéglise C, Marck C, Gaillardin C. The intronome of budding yeasts. C R Biol. 2011;334:662–70 [cited 2019 Apr 15]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/21819948.
Porath HT, Hazan E, Shpigler H, Cohen M, Band M, Ben-Shahar Y, et al. RNA editing is abundant and correlates with task performance in a social bumblebee. Nat Commun. 2019;10:1605 Nature Publishing Group; [cited 2019 May 10]. Available from: http://www.nature.com/articles/s41467-019-09543-w.
Honeybee Genome Sequencing Consortium. Insights into social insects from the genome of the honeybee Apis mellifera. Nature. 2006;443:931–49 [cited 2019 Apr 15]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/17073008.
Feng Q, Hato SV, Langereis MA, Zoll J, Virgen-Slane R, Peisley A, et al. MDA5 detects the double-stranded RNA replicative form in picornavirus-infected cells. Cell Rep. 2012;2:1187–96 [cited 2018 Feb 28]. Available from: http://linkinghub.elsevier.com/retrieve/pii/S2211124712003415.
Mele M, Ferreira PG, Reverter F, DeLuca DS, Monlong J, Sammeth M, et al. The human transcriptome across tissues and individuals. Science (80- ). 2015;348:660–5 [cited 2017 Sep 17]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/25954002.
Kellis M, Wold B, Snyder MP, Bernstein BE, Kundaje A, Marinov GK, et al. Defining functional DNA elements in the human genome. Proc Natl Acad Sci U S A. 2014;111:6131–8 [cited 2019 Apr 15]. Available from: http://www.pnas.org/cgi/doi/10.1073/pnas.1318948111.
Kingsolver MB, Huang Z, Hardy RW. Insect antiviral innate immunity: pathways, effectors, and connections. J Mol Biol. 2013;425:4921–36 [cited 2019 Nov 8]. Available from: https://linkinghub.elsevier.com/retrieve/pii/S0022283613006323.
Chung H, Calis JJA, Wu X, Sun T, Yu Y, Sarbanes SL, et al. Human ADAR1 prevents endogenous RNA from triggering translational shutdown. Cell. 2018;172:811–824.e14 [cited 2018 Feb 19]. Available from: http://linkinghub.elsevier.com/retrieve/pii/S0092867417315180.
Neeman Y, Dahary D, Levanon EY, Sorek R, Eisenberg E. Is there any sense in antisense editing? Trends Genet. 2005;21(10):544-7.
Eisenberg E, Levanon EY. A-to-I RNA editing - immune protector and transcriptome diversifier. Nat Rev Genet. 2018:473–90 [cited 2018 May 6]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/29692414.
Ricci EP, Kucukural A, Cenik C, Mercier BC, Singh G, Heyer EE, et al. Staufen1 senses overall transcript secondary structure to regulate translation. Nat Struct Mol Biol. 2014;21:26–35 [cited 2019 Apr 15]. Available from: http://www.nature.com/articles/nsmb.2739.
Capshew CR, Dusenbury KL, Hundley HA. Inverted Alu dsRNA structures do not affect localization but can alter translation efficiency of human mRNAs independent of RNA editing. Nucleic Acids Res. 2012;40:8637–45 [cited 2019 Apr 15]. Available from: https://academic.oup.com/nar/article-lookup/doi/10.1093/nar/gks590.
Hoffman Y, Dahary D, Bublik DR, Oren M, Pilpel Y. The majority of endogenous microRNA targets within Alu elements avoid the microRNA machinery. Bioinformatics. 2013;29:894–902 [cited 2014 Jul 23]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/23361327.
Reich DP, Tyc KM, Bass BL. C. elegans ADARs antagonize silencing of cellular dsRNAs by the antiviral RNAi pathway. Genes Dev. 2018;32:271–82 [cited 2019 Apr 30]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/29483152.
Feschotte C. Transposable elements and the evolution of regulatory networks. Nat Rev Genet. 2008;9:397–405 [cited 2017 Sep 25]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/18368054.
Tajaddod M, Tanzer A, Licht K, Wolfinger MT, Badelt S, Huber F, et al. Transcriptome-wide effects of inverted SINEs on gene expression and their impact on RNA polymerase II activity. Genome Biol. 2016;17:220 [cited 2018 Nov 4]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/27782844.
Stenger JE, Lobachev KS, Gordenin D, Darden TA, Jurka J, Resnick MA. Biased distribution of inverted and direct Alus in the human genome: implications for insertion, exclusion, and genome stability. Genome Res. 2001;11:12–27 [cited 2019 Apr 29]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/11156612.
Cook GW, Konkel MK, Major JD, Walker JA, Han K, Batzer MA. Alu pair exclusions in the human genome. Mob DNA. 2011;2:10 [cited 2019 Apr 29]. Available from: http://mobilednajournal.biomedcentral.com/articles/10.1186/1759-8753-2-10.
Fujita P, Rhead B, Zweig A, Hinrichs A, Karolchik D, Cline M, et al. The UCSC Genome Browser database. Nucleic Acids Res. 2010;31:51–4 Available from: http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?cmd=Retrieve&db=PubMed&dopt=Citation&list_uids=12519945.
Li H, Durbin R. Fast and accurate short read alignment with Burrows-Wheeler transform. Bioinformatics. 2009;25:1754–60 [cited 2013 Aug 6]. Available from: http://bioinformatics.oxfordjournals.org/cgi/reprint/btp324v1.
Porath HT, Carmi S, Levanon EY. A genome-wide map of hyper-edited RNA reveals numerous new sites. Nat Commun. 2014;5:4726 [cited 2014 Aug 28]. Available from: http://www.nature.com/ncomms/2014/140827/ncomms5726/full/ncomms5726.html%5Cn. http://www.pubmedcentral.nih.gov/articlerender.fcgi?artid=4365171&tool=pmcentrez&rendertype=abstract.
Jun G, Wing MK, Abecasis GR, Kang HM. An efficient and scalable analysis framework for variant extraction and refinement from population-scale DNA sequence data. Genome Res. 2015;25:918–25 Cold Spring Harbor Laboratory Press. [cited 2019 Feb 11]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/25883319.
Li H, Handsaker B, Wysoker A, Fennell T, Ruan J, Homer N, et al. The sequence alignment/map format and SAMtools. Bioinformatics. 2009;25:2078–9 [cited 2018 Aug 12]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/19505943.
Bazak L, Levanon EY, Eisenberg E. Genome-wide analysis of Alu editability. Nucleic Acids Res. 2014;42:6876–84 [cited 2014 Jul 14]. Available from: http://www.pubmedcentral.nih.gov/articlerender.fcgi?artid=4066801&tool=pmcentrez&rendertype=abstract.
Wenric S, ElGuendi S, Caberg J-H, Bezzaou W, Fasquelle C, Charloteaux B, et al. Transcriptome-wide analysis of natural antisense transcripts shows their potential role in breast cancer. Sci Rep. 2017;7:17452.
Eisenberg E, Levanon EY. Human housekeeping genes, revisited. Trends Genet. 2013;29:569–74 [cited 2019 Nov 8]. Available from: http://www.ncbi.nlm.nih.gov/pubmed/23810203.
We thank Brenda L. Bass for the fruitful discussions and critical reading of the manuscript.
We thank the Levanon lab members for the helpful discussions.
Peer review information
Kevin Pang was the primary editor of this article and managed its editorial process and peer review in collaboration with the rest of the editorial team.
The review history is available as Additional file 3.
This work was supported by the JDRF Innovative Grant (1-INO-2018-639-A-N) and the Israel Science Foundation (1380/14) to EYL and Israel Science Foundation (grant numbers 2673/17 and 1945/18) to EE.
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Barak, M., Porath, H.T., Finkelstein, G. et al. Purifying selection of long dsRNA is the first line of defense against false activation of innate immunity. Genome Biol 21, 26 (2020). https://doi.org/10.1186/s13059-020-1937-3