Protein recoding by ADAR1-mediated RNA editing is not essential for normal development and homeostasis
© The Author(s). 2017
Received: 20 June 2017
Accepted: 15 August 2017
Published: 5 September 2017
Adenosine-to-inosine (A-to-I) editing of dsRNA by ADAR proteins is a pervasive epitranscriptome feature. Tens of thousands of A-to-I editing events are defined in the mouse, yet the functional impact of most is unknown. Editing causing protein recoding is the essential function of ADAR2, but an essential role for recoding by ADAR1 has not been demonstrated. ADAR1 has been proposed to have editing-dependent and editing-independent functions. The relative contribution of these in vivo has not been clearly defined. A critical function of ADAR1 is editing of endogenous RNA to prevent activation of the dsRNA sensor MDA5 (Ifih1). Outside of this, how ADAR1 editing contributes to normal development and homeostasis is uncertain.
We describe the consequences of ADAR1 editing deficiency on murine homeostasis. Adar1 E861A/E861A Ifih1 -/- mice are strikingly normal, including their lifespan. There is a mild, non-pathogenic innate immune activation signature in the Adar1 E861A/E861A Ifih1 -/- mice. Assessing A-to-I editing across adult tissues demonstrates that outside of the brain, ADAR1 performs the majority of editing and that ADAR2 cannot compensate in its absence. Direct comparison of the Adar1 -/- and Adar1 E861A/E861A alleles demonstrates a high degree of concordance on both Ifih1 +/+ and Ifih1 -/- backgrounds, suggesting no substantial contribution from ADAR1 editing-independent functions.
These analyses demonstrate that the lifetime absence of ADAR1-editing is well tolerated in the absence of MDA5. We conclude that protein recoding arising from ADAR1-mediated editing is not essential for organismal homeostasis. Additionally, the phenotypes associated with loss of ADAR1 are the result of RNA editing and MDA5-dependent functions.
It is now established that direct RNA modifications, collectively referred to as the epitranscriptome, are widespread, evolutionarily conserved, and contribute significantly to the complexity of gene regulation [1, 2]. A highly prevalent modification is the deamination of adenosine to inosine (A-to-I editing) in double-stranded RNA (dsRNA). A-to-I editing is catalyzed by adenosine deaminase acting on RNA (ADAR) proteins. It is estimated that there are over 100 million potential A-to-I editing sites in humans and tens of thousands in mice [3, 4], with the majority residing within repetitive sequences, such as short interspersed nuclear elements (SINEs), Alus (primates only), and long tandem repeats (LTRs) . Depending on the sequence context—coding sequence, intronic region, untranslated regions, non-coding RNAs—editing can have varying consequences for gene expression . Outside of a small number of examples, the cellular and organismal consequences of A-to-I editing are relatively poorly understood.
Mammals have three ADARs: ADAR (ADAR1), ADARB1 (ADAR2), and ADARB2 (ADAR3); although only ADAR1 and ADAR2 have editing activity in vitro. Physiologically, ADAR2 is essential for the specific editing of a single adenosine in the coding sequence of the glutamate receptor 2 subunit (Gria2) transcript, termed the Q/R site, encoding a neurotransmitter receptor in the brain [7–9]. Inosine is interpreted as guanine by the ribosome so editing of the Gria2 mRNA recodes a genomically encoded glutamine (Q) to arginine (R), varying the permeability of the pore. Adarb1 -/- (Adar2 -/- ) mice cannot edit the Q/R site adenosine, leading to seizures and early lethality. Despite thousands of other editing events identified in both coding and non-coding regions, genomic substitution of the single A to G at the Q/R site rescued the Adar2 -/- phenotype [7, 10]. This result defined the paradigm that RNA editing is a means to post-transcriptionally modify coding sequences and “recode” DNA sequences. Unlike ADAR2, the role of ADAR1 has proven more complex.
ADAR1 is expressed throughout the body, unlike ADAR2 which is highest in the brain . There are two isoforms of ADAR1: a constitutively expressed ADAR1 p110, which is primarily nuclear-restricted, and a longer interferon (IFN) inducible ADAR1 p150, which localizes to both nucleus and cytoplasm . Adar -/- (Adar1 -/- ) mice died at embryonic day 11.5–12.0 (E11.5–12.0) with a profound upregulation of type I IFN and IFN-stimulated genes (ISGs) [13–15]. Likewise, adult somatic deletion of Adar1 resulted in innate immune activation and cell death [14, 16–19]. Mice homozygous for a single amino acid substitution resulting in an editing-deficient ADAR1 protein (Adar1 E861A/E861A ) die at E13.5, with remarkably similar phenotypes to the null allele . Activation of the innate immune sensing system, termed an interferonopathy, is observed in the subset of Aicardi-Goutières syndrome (AGS) patients who harbor mutations in ADAR, demonstrating that the transcriptional response to loss of ADAR1 activity is conserved across mammals [17, 20–22].
In mice and humans, most editing occurs in repetitive sequences capable of base-pairing to form intramolecular dsRNA structures [23–25]. Using murine genetics, we and others demonstrated that editing of endogenous RNA is a critical function of ADAR1, acting to prevent sensing of endogenous (self) dsRNA as foreign [17, 19, 26, 27]. A central function of the innate immune system is the recognition of foreign (non-self) dsRNA by pattern recognition receptors (PRRs) in the cytoplasm. Upon detecting long dsRNA, the PRR melanoma differentiation-associated gene 5 (MDA5, gene name Ifih1) oligomerizes to form a filament leading to activation of mitochondrial antiviral signaling (MAVS), resulting in the production of type I IFN and the propagation of downstream defence signals [28, 29]. Concurrent deletion of MDA5 or MAVS with ADAR1 extended the survival of Adar1 -/- animals until shortly after birth [17, 26]. Viability of the ADAR1 editing-deficient mice was also rescued by deletion of MDA5. These findings suggested that RNA editing is the key function of ADAR1 during early development to prevent activation of MDA5 by endogenous dsRNA.
Editing-dependent and editing-independent functions of ADAR1 have been proposed, including involvement in multiple aspects of microRNA (miRNA) biogenesis [30–35], messenger RNA (mRNA) stability [36, 37], alternate 3’-UTR usage , splicing [38, 39] and translation . Analysis of the Adar1 -/- Mavs -/- and Adar1p150 -/- Mavs -/- rescued mice identified phenotypes associated with the loss of ADAR1 that were considered independent of MAVS/MDA5, including developmental defects in the kidney, small intestine, lymph node, and a failure of B lymphopoiesis . It is unclear if these phenotypes reflect editing-dependent or editing-independent functions of ADAR1.
Due to embryonic lethality of the Adar1 -/- and Adar1 E861A/E861A mice, establishing the in vivo relevance of ADAR1’s functions to adult homeostasis had not been possible. In contrast to the Adar1 -/- Ifih1 -/- or Adar1 -/- Mavs -/- that die within days of birth, the Adar1 E861A/E861A Ifih1 -/- survived until at least four weeks of age . We have assessed the requirement for ADAR1 activity during adult murine homeostasis using these rescued ADAR1 editing-deficient animals. We directly compared the Adar1 -/- and Adar1 E861A alleles, on both a Ifih1 +/+ and Ifih1 -/- background, on the day of birth and in an acute adult somatic mutation model to evaluate editing-independent functions of ADAR1. We conclude that the core function of ADAR1-mediated editing is to prevent the formation of MDA5 substrates and that other effects of ADAR1-mediated editing, such as protein recoding and on miRNA biology, are not essential for murine homeostasis in vivo.
Adar1E861A/E861AIfih1-/- animals have a normal lifespan and low weaning weight
Mild innate immune activation in the absence of MDA5
The protein levels of eight cytokines/chemokines in peripheral blood (PB) serum that increased upon somatic deletion of Adar1 were assessed . There was no increase in any of the proteins assessed including IFNβ, IFNγ, CCL2, and CXCL10 (Fig. 2b). The only difference was an Ifih1 -/- genotype-dependent reduction in the expression of CCL11 (Fig. 2b). As a positive control, the expression of these proteins was assessed in supernatant from cultures of immortalized hematopoietic cells , generated from R26-CreERT2 Adar1 E861A/fl bone marrow (BM) cells, treated with tamoxifen in vitro (Fig. 2b). Despite the increased ISG mRNAs there is no resultant increase in circulating protein levels.
Normal hematopoiesis in the absence of ADAR1-mediated A-to-I editing
Within the BM, relatively mild and subtle changes were apparent that reflected the PB. Total BM cellularity and myeloid development was essentially normal between genotypes (Fig. 3f, g). Analysis of B-cell differentiation demonstrated that the lower B-cell numbers in the Adar1 +/+ Ifih1 -/- stemmed from a reduction of cells at the ProB cell stage (Fig. 3h). Consistent with the Ifih1 -/- -dependent anemia, there were reduced numbers of mature CD71-Ter119+ erythroid cells in the BM of animals with this genotype (Fig. 3i). In the stem and primitive progenitor populations, there were relatively subtle differences among the groups, but in all cases the numbers of each population were largely normal (Fig. 3j, k). Hematopoiesis in the spleen (Fig. 3l) and thymus (Fig. 3m) was normal compared to controls. ADAR1-mediated editing in not required for homeostatic hematopoiesis once MDA5 is inactivated.
Normal tissue development in the absence of ADAR1-mediated A-to-I editing
Due to the reduced weaning weight and requirement for ADAR1 in bone/osteoblast homeostasis , we quantitated the bone parameters in 12-week-old Adar1 E861A/E861A Ifih1 -/- animals compared to controls by microCT . Both male and female mice were assessed; however, due to variability in bone indices with estrus in females, we focused our analysis on the males (female data in Additional file 3: Figure S1). The total tibial length and trabecular bone parameters were normal in the Adar1 E861A/E861A Ifih1 -/- animals (Fig. 4b–g). The only significant differences were modest changes in the cortical thickness (Fig. 4h, i) and cortical area (Fig. 4j) between the Adar1 E861A/E861A Ifih1 -/- animals and the C57BL/6 and Adar1 +/+ Ifih1 -/- animals. There was a reduced endocortical perimeter when the Adar1 E861A/E861A Ifih1 -/- were compared to the Adar1 +/+ Ifih1 -/- animals (Fig. 4k), but not to the C57BL/6 s. Therefore, ADAR1-mediated A-to-I editing is dispensable for normal organ and skeletal development once MDA5 is inactivated.
Transcriptome analysis of whole brain from adult rescued mice
ADAR1 is the primary editing enzyme in peripheral tissue and editing levels are significantly reduced in the Adar1E861A/E861AIfih1-/- tissues
A-to-I editing across a range of defined substrates was assessed using microfluidics multiplexed PCR and deep sequencing (mmPCRseq) , allowing accurate measurements of editing of up to 11,103 sites in 557 loci (Fig. 6a–h, lower panels, Additional file 5: Dataset S3). Changes in editing across the tissues principally reflected the expression profile of Adar1 and Adar2. In the brain, where there are higher relative levels of Adar2 than Adar1, there is a largely preserved editome with evidence for a subset of ADAR1-specific and ADAR2-specific events (dots on y-axis or x-axis, respectively), but the majority can be edited by both. In contrast, in hematopoietic tissues there is little/no detectable Adar2 and with this there is a near complete absence of editing of known sites when ADAR1 editing is inactivated. In other peripheral tissues assessed, Adar1 predominates and most editing of known sites was lost in the Adar1 E861A/E861A -derived samples. Examples for ADAR1-specific, ADAR2-specific, and ADAR1/2 shared editing sites were observed (Fig. 6i). We further assessed the status of evolutionary conserved recoding events across the tissues . The most informative tissue was the brain, where the majority of these transcripts were robustly expressed (Fig. 6j). In the brain, editing at most sites was preserved indicating that ADAR2 was editing these sites. Known ADAR1 dependent sites such as Bclap and two sites in the Htr2c transcript had significantly reduced/no editing in the brain [13, 50]. For the remaining tissues, there were several patterns apparent: the transcripts were not detected as expressed in the tissue assessed (indicated in white; see Additional file 5: Dataset S3 for mouse ENCODE expression data from tissues for each transcript); that editing of the conserved sites was preserved indicating an ADAR2-specific target, even in tissue with relatively low levels of Adar2 as assessed by qPCR (see Cog3 as an example); that there was a loss of editing at these sites in the Adar1 E861A/E861A Ifih1 -/- -derived tissues indicating these sites are ADAR1-dependent (see Kcna1 in the liver, Nova1 in the bone marrow, Cyfip2 in the liver and small intestine for examples). The failure to edit the conserved sites in the Adar1 E861A/E861A Ifih1 -/- tissues suggests that while they are ADAR1-dependent sites, their absence was not deleterious. This analysis demonstrated that editing in the tissues outside the central nervous system that were assessed is primarily mediated by ADAR1, yet despite the loss of this editing, these tissues are normal in the absence of MDA5.
The absence of ADAR1 or loss of ADAR1-mediated A-to-I editing are equivalent in vivo
Next, we evaluated this using an acute somatic deletion model comparing R26-CreER Adar1 fl/+ (control; expressing WT ADAR1 protein after tamoxifen treatment), R26-CreER Adar1 fl/fl (ADAR1 protein null after tamoxifen treatment), and R26-CreER Adar1 fl/E861A (expressing an editing deficient ADAR1 protein after tamoxifen treatment) on both an MDA5 WT and null background (Fig. 7c). All mice were aged at least eight weeks at the initiation of up to 28 days treatment with tamoxifen administered via the food (400 mg/kg in standard chow). The R26-CreER Adar1 fl/fl and R26-CreER Adar1 fl/E861A animals both lost condition and weight from day 14 onward (Fig. 7d–f). This decline in health was accompanied by a severe reduction in PB indices and the euthanasia of all R26-CreER Adar1 fl/E861A animals and three of four R26-CreER Adar1 fl/fl animals prior to day 28 of treatment (Fig. 7f, g). All remaining genotypes remained healthy at day 28 and were assessed on day 29 (Fig. 7d). Upon euthanasia or cessation of tamoxifen as indicated, genotyping confirmed the efficient recombination of the floxed allele in the R26-CreER Adar1 fl/+ animals (Fig. 7e). The R26-CreER Adar1 fl/fl and R26-CreER Adar1 fl/E861A , while both moribund and requiring euthanasia, retained the floxed allele indicative of selection against deletion as previously observed in other settings [14, 18, 19]. Strikingly, the absence of MDA5 allowed the efficient recombination of the floxed allele in both the R26-CreER Adar1 fl/fl Ifih1 -/- and R26-CreER Adar1 fl/E861A Ifih1 -/- animals (Fig. 7e).
We focused our assessment on hematopoiesis, given the well-characterized impact of ADAR1 deficiency on this system. Across PB (Fig. 7g), BM (Fig. 7h–m), spleen (Fig. 7n, Additional file 3: Figure S2), and thymus (Fig. 7o, Additional file 3: Figure S2), the results were highly comparable: that the complete absence of ADAR1 protein and the specific absence of A-to-I editing by ADAR1 were largely indistinguishable, and that the deletion of MDA5 rescued both the ADAR1 null and editing deficient alleles equivalently. In the presence of MDA5, the deletion of ADAR1 or prevention of editing by ADAR1 resulted in a loss of erythroid progenitors (Fig. 7j), a block in B-cell maturation in the BM (Fig. 7k), an accumulation of phenotypic stem and primitive progenitor populations (Fig. 7l) with a loss of the committed myelo-erythroid progenitor populations (Fig. 7m). These changes were prevented by the deletion of MDA5. The activation status of the innate immune response was queried using expression of Sca1, a cell surface protein induced by IFN resultant from an innate immune response [14, 51]. In the R26-CreER Adar1 fl/fl and R26-CreER Adar1 fl/E861A BM primitive hematopoietic population, there was a profound upregulation of Sca1 expression that was completely prevented by deletion of MDA5 (Fig. 7p). Intestinal length was assessed as prior work identified intestinal shortening following the somatic deletion of Adar1 in a Mavs -/- background, although the age of these animals was not provided . No difference in intestinal length was observed in our cohorts (Fig. 7q). These results demonstrate that the complete absence of ADAR1 and the specific absence of ADAR1-mediated A-to-I editing, in either the presence or absence of MDA5, respectively, are largely indistinguishable in adult mice. Therefore, preventing MDA5 substrate formation requires A-to-I editing of endogenous RNA and is the primary in vivo function of ADAR1.
The consequences of altered ADAR1 function are severe, from embryonic lethality in mice to debilitating neurological disease and systemic interferonopathy in humans with loss-of-function alleles [22, 52], to putative oncogenic roles when overexpressed [31, 53, 54], so it is critical to clearly define the key function(s) of ADAR1. In contrast to the physiologically essential role of transcript recoding by ADAR2, the importance of recoding to the biology of ADAR1 was unknown. In addition to protein recoding, ADAR1 can edit dsRNA substrates resulting in changes in multiple aspects of miRNA biogenesis or function, affect mRNA stability, 3’-UTR length and translation, and modify splice site usage in addition to altering dsRNA secondary structures, which have been proposed to interface with the innate immune sensing system [19, 55]. We now demonstrate that the absence of ADAR1-mediated editing is surprisingly well tolerated, once the innate immune sensor MDA5 is deleted. Adar1 E861A/E861A Ifih1 -/- mice are strikingly normal in a homeostatic state. Given the extent of A-to-I editing in the transcriptome, the precedent of ADAR2/Gria2 and the diverse functions in which ADAR1 is implicated [2, 6, 56, 57], this was unexpected. This demonstrates that exonic recoding of transcripts by ADAR1, as well as other proposed editing-dependent effects of ADAR1 on gene expression, are not essential for development and adult homeostasis. Consistent with this, we saw very few changes to the global gene expression profile in adult brain of Adar1 E861A/E861A Ifih1 -/- mice. The lack of phenotypes in the Adar1 E861A/E861A Ifih1 -/- mice at homeostasis reveals that ADAR1’s primary and physiologically most important function is to edit endogenous RNA to prevent the formation of endogenous MDA5 substrates.
We do not exclude subtle or additional phenotypes in the Adar1 E861A/E861A Ifih1 -/- mice that were not appreciated in our analysis, as were demonstrated after the broad phenotypic testing of the Adar2 -/- Gria2 R/R mice . Additionally, the analysis of the Adar1 E861A/E861A Ifih1 -/- animals in non-homeostatic settings, such as when subjected to stress or in pathological settings, may identify essential functions for ADAR1-mediated editing that are not apparent under the homeostatic conditions assessed here. A small number of mammalian conserved, positively selected recoding events have been identified . While ADAR2 can edit many of these sites, particularly in the brain, it is also highly likely that the requirement for these may only become apparent in very specific circumstances. The known conserved ADAR1 dependent sites in Bclap and the Htr2c transcript were no longer edited in the Adar1 E861A/E861A Ifih1 -/- animals. Recoding events mediated by ADAR1 have been demonstrated to result in altered protein function. An example is the recoding of a serine-to-glycine in AZIN1 (p.S365G) [49, 54]. In this instance, the edited form of AZIN1 is predicted to result in a gain-of-function allele, whereas our murine models have a loss of ADAR1-mediated editing and the physiological consequences of this are likely to be distinct. Overall, the absence of the conserved ADAR1-mediated recoding events appears well tolerated, suggesting that these proteins may have functions in the whole organism that are either mild/subtle, that their absence is not sufficient to be pathogenic in isolation, or that these only demonstrate an essential requirement in specific settings.
The nexus between ADAR1 and the innate immune system, centered on the MDA5-MAVS axis, has solidified due to the work of a number of groups, including our own [17, 26]. However, the differences between the Adar1 E861A/E861A Ifih1 -/- animals reported here and the various Adar1 -/- rescued mice are intriguing . Mannion et al. reported survival of the Adar1 -/- Mavs -/- animals until the day of birth and that there was normal histology of internal organs of an Adar1 -/- Mavs -/- pup at this time . Pestal et al. also identified that the vast majority (>90–95%) of both Adar1 -/- Mavs -/- and Adar1 -/- Ifih1 -/- pups died by two days after birth. A very small number of the Adar1 -/- Mavs -/- pups were identified that survived for 13–20 days. These rare Adar1 -/- Mavs -/- survivors had defects in kidney patterning, small intestines, lymph nodes, and B lymphopoiesis . The Adar1 E861A/E861A Ifih1 -/- animals do not have these phenotypes, nor is an absence of B cells apparent in the cohort of Adar1 -/- Ifih1 -/- pups we assessed on the day of birth (Fig. 7a, b). The simplest interpretation of this is that editing-independent functions of ADAR1 have essential functions, specifically in early post-natal development. The phenotypes reported for the rescued Adar1 -/- were on a Mavs -/- background, which may be an important contributing factor to the differences compared to the Adar1 E861A/E861A Ifih1 -/- . The genetic rescue of the Adar1 -/- achieved by loss of MDA5 was qualitatively better than MAVS deficiency at the day of birth . A possible explanation may be that there is a difference between the cellular consequences of being Mavs -/- and Ifih1 -/- . In Adar1 -/- Mavs -/- and Adar1p150 -/- Mavs -/- cells, unedited endogenous dsRNA – the presumptive candidate immunogenic substrate – are formed and can be sensed by MDA5. The loss of MAVS prevents downstream signaling, but sensing and filament formation by MDA5 remains intact. While the consequences of MDA5 filament formation in the absence of signaling is unknown, it is possible based on the rescue of the Adar1 E861A/E861A Ifih1 -/- animals and cells that these may in part contribute to the phenotypes observed. Supporting this, in a cell-based assay of MDA5 function, 5–10% of signaling activity remained in the absence of MAVS .
To directly assess the contribution of editing-dependent and editing-independent function of ADAR1 under identical conditions, we assessed pups at the day of birth and used an adult somatic deletion model that leaves animals acutely as either Adar1-null (Adar1 fl/fl ) or editing deficient (Adar1 fl/E861A ). The pups assessed on the day of birth were grossly normal, had normal B cell frequency in the spleen, and no evidence of activated ISGs, indicating that an absence of B cells is not an MDA5-independent function of ADAR1 at the age assessed but may be a phenotype restricted to those rare animals that survived 10–20 days after birth . How these rare Adar1 -/- Mavs -/- animals adapted and survived is unclear. ADAR1p150 appears to have a more specific function in B-cell homeostasis than ADAR1p110 based on the analysis of Adar1p150 -/- Mavs -/- , which would not be appreciable in the assays we have completed where both ADAR1 isoforms are either null or editing deficient . In the somatic deletion model that we have applied, there was no/little difference across nearly all cell populations enumerated between the being ADAR1 null and editing-deficient on either an MDA5 WT and null background. This demonstrated that the Adar1-null animals were no worse off than animals expressing only an editing-deficient protein. Second, the phenotypes of ADAR1 deficiency or of editing loss were comparably rescued by MDA5 deletion. The somatic deletion of Adar1 on a Mavs -/- background resulted in disrupted intestinal homeostasis five days after tamoxifen treatment , with the caveat that the Adar1 +/+ Mavs -/- control was not described. This was not observed in the experiments that we completed using the adult deletion model on an Ifih1 -/- background; however, these experiments have several important differences including Cre strain used and route of tamoxifen administration that limit direct comparison.
While acknowledging there may be editing-independent functions of ADAR1 that are only apparent in early postnatal development, we favor an alternative interpretation. We hypothesize a critically sensitive time point in early post-natal development where unedited dsRNA loads reach a high enough level, akin to the threshold model proposed for DNA sensing , that development cannot proceed and where having an ADAR1 protein, even editing-deficient, that can bind RNA is sufficient to “sequester” the dsRNA, can block/reduce signaling to a tolerated level. Whether expression of an editing-deficient cytosolic isoform of ADAR1 would elicit the same effect requires testing. If it were to reduce innate immune signaling in the absence of editing, it would support the concept as has been observed in C. elegans and in murine embryonic fibroblasts (MEFs) [26, 60]. The subtle innate immune activation, at least on a transcriptional level in the Adar1 E861A/E861A Ifih1 -/- tissues, alludes to alternative minor pathways able to induce the production of ISGs independent of MDA5 (Fig. 2a). Very recently it was reported that Ribonuclease L deficiency could rescue cell death associated with deletion of ADAR1 in a human cell line model . The murine genetic data and rescue indicate that such a mechanism does not get activated in the Adar1 E861A/E861A Ifih1 -/- animals, consistent with the concept that having a protein capable of binding RNA, even if incapable of editing, is advantageous compared to being completely deficient for ADAR1.
The present data demonstrate that once MDA5 is neutralized, there are no essential ADAR1-mediated editing events required for mammalian development and adult homeostasis. We do not find evidence for an analogous essential protein recoding event(s) mediated by ADAR1 to that of Gria2 for ADAR2. Moreover, A-to-I editing by ADAR1 of a variety of substrates, including the editing of miRNAs and their target sequences, outside of modifying the potential for these to interact with MDA5, is neither essential nor required for normal mammalian homeostasis. The parallels between the ADAR1 null and editing-deficient models suggest that editing independent roles of ADAR1 are not significant contributors to the in vivo phenotypes associated with loss of ADAR1. As the transcriptional response and cellular consequences of loss of ADAR1 are conserved across mammals, these data have implications for humans with ADAR1 mutations, particularly those with AGS [17, 21, 52]. Our data demonstrate that if MDA5 activity/expression can be prevented or reduced, even in the context of a completely editing-deficient ADAR1 protein, this is sufficient to result in largely normal development with limited consequences on long-term organ and tissue homeostasis.
These analyses demonstrate that the lifetime absence of ADAR1-editing is well tolerated, once MDA5 is inactivated. We conclude that protein recoding arising from ADAR1-mediated editing, unlike ADAR2, is not essential for organismal homeostasis. The comparison of both germline and acute somatic deficient Adar1 -/- and Adar1 E861A animals, on either a WT and MDA5-deficient background, did not identify distinct differences between being ADAR1 protein-deficient and having only the expression of an editing dead protein. The phenotypes associated with loss of ADAR1 are the result of RNA editing and MDA5-dependent functions. A-to-I editing by ADAR1 of a variety of substrates, including the editing of miRNAs and their target sequences, outside of modifying the potential for these to interact with MDA5, is neither essential nor required for normal mammalian homeostasis.
All animal experiments were approved by the AEC (AEC#030/14 and AEC#031/15; St. Vincent’s Hospital, Melbourne). Adar E861A/+ (Adar1 E861A/+ ; MGI allele: Adar tm1.1Xen ; MGI:5805648), Ifih1 -/- (Ifih1 tm1.1Cln ), Adar -/- (Adar1 -/- ; MGI allele: Adar tm2Phs ; MGI:3029862), Adar fl/fl (Adar1 fl/fl ; MGI allele: Adar tm1.1Phs ; MGI:3828307), and Rosa26-CreERT2 (Gt(ROSA)26Sortm1(cre/ERT2)Tyj) mice were on a backcrossed C57BL/6 background as previously described [14, 18, 19, 62, 63]. For day of birth analysis, females were plug mated and pups collected before midday on the day of birth. For acute somatic deletion model, all animals were aged ≥ 8 weeks at tamoxifen initiation; tamoxifen-containing food was prepared at 400 mg/kg tamoxifen citrate (Sigma) in standard mouse chow (Specialty Feeds, WA, Australia).
Four (two males, two females) 12-week-old Adar1 E861A/+ Ifih1 -/- and Adar1 E861A/E861A Ifih1 -/- littermates were used for histopathology examination. Tissue collection and histology was performed by the Australian Phenomics Network Histopathology and Organ Pathology Core, University of Melbourne. One male and one female Adar1 E861A/+ Ifih1 -/- were genotype identified to the pathologists as “controls,” the remaining samples were genotype blinded. Sections were assessed by independent pathologists. The full pathology report is available in Additional file 3: Dataset S1.
Flow cytometry analysis and fluorescent activated cell sorting
Peripheral blood was analyzed on a hematological analyzer (Sysmex KX-21 N, Roche Diagnostics). Single-cell BM, spleen, and thymus suspensions were prepared by passing through a 23-G needle (BM) or crushing through a 40-μm cell strainer (spleen/thymus) . Antibodies against murine Ter119, CD71, B220, IgM, CD11b/Mac1, Gr1, F4/80, CD43, CD19, CD4, CD8, CD44, Sca-1, c-Kit, CD34, FLT3, FcγR (CD16/32), CD41, CD105, and CD150 were either biotinylated or conjugated with FITC; phycoerythrin, phycoerythrin-Cy5, peridinin chlorophyll protein-Cy5.5, phycoerythrin-Cy7, allophycocyanin, or allophycocyanin eFluor780 were all obtained from eBioscience. CD105 and CD150 were from BioLegend. Biotinylated antibodies were detected with streptavidin conjugated with Brilliant Violet-605 (Biolegend). Cells were analyzed on a BD LSRIIFortessa (BD Biosciences). Results were analyzed with FlowJo software Version 10.0 (Treestar).
For serum cytokine/chemokine expression analysis, serum was isolated from peripheral blood and assessed using a custom bead-based immunoassay (LEGENDPlex, BioLegend) measuring murine IFNγ IFNβ, IL-10, TNFα, CXCL10, CXCL1, CCL2, and CCL11. Serum from age- and sex-matched WT C57B6/J mice from the same rooms of the BioResources Facility were run in parallel. Samples were assessed on BD LSRIIFortessa (BD Biosciences). Results were analyzed with LEGENDPlex software version 7.0 (Biolegend). As a control, tissue culture media was isolated from immortalized myeloid progenitor cells generated from Rosa26-CreERT2 Adar1 E861A/fl cell lines that were treated with 200 nM tamoxifen for four days to delete the WT Adar1 allele. These cells were immortalized with HoxA9 and selected for proliferation in GM-CSF conditioned media as described .
Micro-computed tomography analysis of bone parameters (microCT)
Ex vivo microCT was performed on tibiae using the SkyScan1076 system (Bruker-microCT, Kontich, Belgium) essentially as previously described . Male and female 12-week-old tibia were isolated, fixed overnight in 2% paraformaldehyde, and then stored in 70% ethanol until imaged. Images were acquired using the following settings: pixel size = 9 μm, aluminum filter = 0.5 mm, voltage = 45 kV, current = 220 μA, rotation = 0.7°, and frame averaging = 1. Images were reconstructed and analyzed with SkyScan software programs NRecon (version 220.127.116.11), DataViewer (version 1.4.4), CT Analyser (CTan, version 18.104.22.168), and CTVox (version 2.2.0). The trabecular analysis region of interest (ROI) was determined by identifying the start of the mineralized zone of the proximal growth plate and calculating 3% of the total tibial length towards the tibial mid-shaft, where we then analyzed an ROI of 13.5% of the total tibial length. Analysis of trabecular bone structure was completed using adaptive thresholding (mean of min and max values) in CTan with threshold set at 45–255 for trabecular bone. Cortical analyses were performed at 40% of the total tibial length distal from the mineralized zone of the proximal growth plate and extending for 13.5% of the total tibial length; the threshold values for cortical bone were set to 79–255 and global thresholding algorithm was used. The three-dimensional visualization of trabecular and cortical bone was performed with CTVox, where volume-rendered images were pseudo-colored based on grayscale (pixel) intensity that is reflective of bone mineralization.
Mouse tissues from three independent biological replicates from age-matched and sex-matched C57BL/6, Adar1 +/+ Ifih1 -/- , and Adar1 E861A/E861A Ifih1 -/- mice were homogenized in Trisure reagent using IKA T10 basic S5 Ultra-turrax Disperser. Brain tissue was isolated from the pups collected at the day of birth and snap-frozen, then homogenized in Trisure reagent using IKA T10 basic S5 Ultra-turrax Disperser. RNA was extracted using Direct-Zol columns (Zymo Research) as per manufacturer’s instructions. Complementary DNA (cDNA) was synthesized using Tetro cDNA synthesis kit (Bioline). Real-time PCR was done in duplicate with Brilliant II SYBR Green QPCR Master Mix (Agilent Technologies) and primers from IDT (Additional file 3: Table S2). All primers were optimized to have equal efficiency (100+/-10%) before use. Ppia was used as a reference gene for relative quantification using the ∆Ct method. RNA was obtained from fetal brain from E12.5 Adar1 E861A/E861A embryos and processed as described above .
Microfluidics-based multiplex PCR and deep sequencing (mmPCR-seq) identification of A-to-I editing sites
Whole brain, kidney, spleen, thymus, BM, heart, and small intestines from three independent biological replicates from Adar1 +/+ Ifih1 -/- and Adar1 E861A/E861A Ifih1 -/- were used for mmPCR-seq. Following tissue homogenization, RNA was isolated using TRIsure reagent (Bioline) and Direct-Zol columns (Zymo Research). cDNA was synthesized using iScript Advanced Kit (BioRad) using 1.2–7.5 μg RNA per tissue. A total of 200 ng of cDNA was used for mmPCR-seq targeting 557 loci containing 11,103 known A-to-I editing sites . A-to-I editing frequency was assessed using the criteria: minimum coverage > 100 (in 2/3) of WT (Adar1 +/+ Ifih1 -/- ) and deficient (Adar1 E861A/E861A Ifih1 -/- ). For a given site, where a replicate had ≤ 100 reads that measurement is regarded as a missing value. All editing sites with editing ≤ 0.01 were removed, leaving 413–808 sites per tissue. Sites were ADAR1-specific targets if the editing level measurements between the WT (Adar1 +/+ Ifih1 -/- ) replicates and the editing-deficient (Adar1 E861A/E861A Ifih1 -/- ) replicates were significantly different (P < 0.1, ANOVA) and the average editing levels between WT and editing-deficient samples differed by at least 5% .
RNA-seq samples: adult brain
Total RNA was isolated from the whole brain from 12-week-old male Adar1 +/+ Ifih1 -/- and Adar1 E861A/E861A Ifih1 -/- mice (n = 3/genotype). Sequins were included before ribosome depletion . Post ribosome-depleted RNA was purified and subjected to indexing and library preparation using the Kapa Stranded RNA-seq Library Preparation Kit (Kapa Biosystems) and sequenced using the Illumina NextSeq500 with 75-bp paired-end reads by the Ramaciotti Centre for Genomics (UNSW, Australia).
RNA-seq samples: fetal brain
Total RNA was isolated from the whole brain from E12.5 old male Adar1 +/+ Ifih1 -/- and Adar1 E861A/E861A Ifih1 -/- mice (n = 3/genotype). RNA was purified and subjected to indexing and library preparation using the Illumina TruSeq RNA Sample Prep Kit v2. The libraries were sequenced using the Illumina HiSeq2000 with 100-bp paired-end reads by the Ramaciotti Centre for Genomics (UNSW, Australia).
RNA-seq reads from adult brain were aligned to the MM9/NCBIM37 reference genome with STAR  and gene counts were determined using “--quantMode GeneCounts.” Differential gene expression analysis was performed using the Degust analysis tool (http://victorian-bioinformatics-consortium.github.io/degust/); briefly, genes were only considered with a CPM of ≥ 2 in 3/3 replicates of either the Adar1 E861A/E861A Ifih1 -/- or Adar1 +/+ Ifih1 -/- (13,891 genes). Normalized read counts (moderated log counts per million) and differential expression were generated using edgeR  and genes were considered differentially expressed if FDR < 0.05 (124 genes: 81 up, 43 down). Adding a magnitude requirement to the fold change of abs(log2FC) > 1 resulted in 29 genes (24 up, 5 down).
RNA-seq reads from fetal brain were aligned to the MM9/NCBIM37 reference genome with STAR  and gene counts were determined using “--quantMode GeneCounts.” Differential gene expression analysis was performed using the Degust analysis tool (http://victorian-bioinformatics-consortium.github.io/degust/); briefly, genes were only considered with a CPM of ≥ 2 in 3/3 replicates of either the Adar1 E861A/E861A Ifih1 -/- or Adar1 +/+ Ifih1 -/- (13,786 genes). Normalized read counts (moderated log counts per million) and differential expression were generated using edgeR  and genes were considered differentially expressed if FDR < 0.05 (808 genes: 745 up, 57 down). Adding a magnitude requirement to the fold change of abs(log2FC) > 1 resulted in 303 genes (294 up, 9 down).
GO term enrichment of genes using PANTHER
PANTHER Overrepresentation Test  (release 20160715): PANTHER version 11.1 was used to perform statistical testing on sets of differential genes using all Mus musculus genes as the reference list against GO biological processes, using Bonferroni multiple testing correction.
QuSAGE gene set testing
Quantitative Set Analysis for Gene Expression (QuSAGE) was performed as described  against the MSigDB collection “C2:curated gene sets” (c2.cgp.v4.0).
All datasets related to this work are deposited in GEO.
GSE94387 (adult brain)
GSE94388 (fetal brain)
GSE94386 (mmPCR-seq: BM, spleen, thymus, liver, brain, kidney, small intestine, and heart)
For biological experiments, the significance of results was analyzed using the one-way or two-way ANOVA with multiple comparison corrections unless otherwise stated, P < 0.05 was considered significant. All data are presented as mean ± SEM.
We thank B. Tonkin for technical assistance; T. Mercer (Garvan Institute) for sequins; J. Hartner, T. Sun, and L. Purton for their comments/discussion. We also thank SVH BioResources Centre, SVI Flow Cytometry Facility (M. Thomson), APN Histopathology and Organ Pathology Service, University of Melbourne.
This work was supported by grants an NHMRC (APP1102006; CW and JBL), Angior Foundation Grant (CW), SVI Women in Research Award (JHF), NIH R01GM102484 (JBL), Ellison Medical Foundation (JBL), Stanford University Department of Genetics (JBL); in part by the Victorian State Government OIS (to St. Vincent’s Institute); Victorian Cancer Agency Mid-Career Fellowship (MCRF15015; CW).
Availability of data and materials
The datasets generated and analyzed during the current study are available in GEO.
RNA-seq accessions: GSE94387 (adult brain); GSE94388 (fetal brain); GSE94386 (mmPCR-seq: BM, spleen, thymus, liver, brain, kidney, small intestine, and heart).
JHF, AMC, SEL, QL, ST, JW, LP, BL, AG, JBL, and CRW performed experiments, analyzed and interpreted data; JHF, JBL, and CRW provided intellectual input and conceptual advice; JHF and CRW wrote the manuscript. All authors read and approved the final manuscript.
Ethics approval and consent to participate
All animal experiments were approved by the St. Vincent’s Hospital, Melbourne Animal Ethics Committee (AEC#030/14 and AEC#031/15).
Consent for publication
The authors declare that they have no competing interests.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Open AccessThis 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.
- Gilbert WV, Bell TA, Schaening C. Messenger RNA modifications: Form, distribution, and function. Science. 2016;352:1408–12.View ArticlePubMedPubMed CentralGoogle Scholar
- O’Connell MA, Mannion NM, Keegan LP. The epitranscriptome and innate immunity. PLoS Genet. 2015;11:e1005687.View ArticlePubMedPubMed CentralGoogle Scholar
- 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.View ArticlePubMedPubMed CentralGoogle Scholar
- Ramaswami G, Li JB. RADAR: a rigorously annotated database of A-to-I RNA editing. Nucleic Acids Res. 2014;42:D109–113.View ArticlePubMedGoogle Scholar
- Hundley HA, Bass BL. ADAR editing in double-stranded UTRs and other noncoding RNA sequences. Trends Biochem Sci. 2010;35:377–83.View ArticlePubMedPubMed CentralGoogle Scholar
- Nishikura K. A-to-I editing of coding and non-coding RNAs by ADARs. Nat Rev Mol Cell Biol. 2016;17:83–96.View ArticlePubMedGoogle Scholar
- Higuchi M, Maas S, Single FN, Hartner J, Rozov A, Burnashev N, et al. Point mutation in an AMPA receptor gene rescues lethality in mice deficient in the RNA-editing enzyme ADAR2. Nature. 2000;406:78–81.View ArticlePubMedGoogle Scholar
- Higuchi M, Single FN, Kohler M, Sommer B, Sprengel R, Seeburg PH. RNA editing of AMPA receptor subunit GluR-B: a base-paired intron-exon structure determines position and efficiency. Cell. 1993;75:1361–70.View ArticlePubMedGoogle Scholar
- Sommer B, Kohler M, Sprengel R, Seeburg PH. RNA editing in brain controls a determinant of ion flow in glutamate-gated channels. Cell. 1991;67:11–9.View ArticlePubMedGoogle Scholar
- Horsch M, Seeburg PH, Adler T, Aguilar-Pimentel JA, Becker L, Calzada-Wack J, et al. Requirement of the RNA-editing enzyme ADAR2 for normal physiology in mice. J Biol Chem. 2011;286:18614–22.View ArticlePubMedPubMed CentralGoogle Scholar
- Huntley MA, Lou M, Goldstein LD, Lawrence M, Dijkgraaf GJ, Kaminker JS, et al. Complex regulation of ADAR-mediated RNA-editing across tissues. BMC Genomics. 2016;17:61.View ArticlePubMedPubMed CentralGoogle Scholar
- Liu Y, George CX, Patterson JB, Samuel CE. Functionally distinct double-stranded RNA-binding domains associated with alternative splice site variants of the interferon-inducible double-stranded RNA-specific adenosine deaminase. J Biol Chem. 1997;272:4419–28.View ArticlePubMedGoogle Scholar
- Hartner JC, Schmittwolf C, Kispert A, Muller AM, Higuchi M, Seeburg PH. Liver disintegration in the mouse embryo caused by deficiency in the RNA-editing enzyme ADAR1. J Biol Chem. 2004;279:4894–902.View ArticlePubMedGoogle Scholar
- 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.View ArticlePubMedGoogle Scholar
- Wang Q, Miyakoda M, Yang W, Khillan J, Stachura DL, Weiss MJ, et al. Stress-induced apoptosis associated with null mutation of ADAR1 RNA editing deaminase gene. J Biol Chem. 2004;279:4952–61.View ArticlePubMedGoogle Scholar
- XuFeng R, Boyer MJ, Shen H, Li Y, Yu H, Gao Y, et al. ADAR1 is required for hematopoietic progenitor cell survival via RNA editing. Proc Natl Acad Sci U S A. 2009;106:17763–8.View ArticlePubMedPubMed CentralGoogle Scholar
- 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.View ArticlePubMedPubMed CentralGoogle Scholar
- Liddicoat BJ, Hartner JC, Piskol R, Ramaswami G, Chalk AM, Kingsley PD, et al. Adenosine-to-inosine RNA editing by ADAR1 is essential for normal murine erythropoiesis. Exp Hematol. 2016;44:947–63.View ArticlePubMedGoogle Scholar
- 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. 2015;349:1115–20.View ArticlePubMedPubMed CentralGoogle Scholar
- Rice GI, del Toro DY, Jenkinson EM, Forte GM, Anderson BH, Ariaudo G, et al. Gain-of-function mutations in IFIH1 cause a spectrum of human disease phenotypes associated with upregulated type I interferon signaling. Nat Genet. 2014;46:503–9.View ArticlePubMedPubMed CentralGoogle Scholar
- Rice GI, Kasher PR, Forte GM, Mannion NM, Greenwood SM, Szynkiewicz M, et al. Mutations in ADAR1 cause Aicardi-Goutieres syndrome associated with a type I interferon signature. Nat Genet. 2012;44:1243–8.View ArticlePubMedPubMed CentralGoogle Scholar
- Rice GI, Kitabayashi N, Barth M, Briggs TA, Burton AC, Carpanelli ML, et al. Genetic, phenotypic, and interferon biomarker status in ADAR1-related neurological disease. Neuropediatrics. 2017;48:166–84.View ArticlePubMedGoogle Scholar
- Ramaswami G, Lin W, Piskol R, Tan MH, Davis C, Li JB. Accurate identification of human Alu and non-Alu RNA editing sites. Nat Methods. 2012;9:579–81.View ArticlePubMedPubMed CentralGoogle Scholar
- Danecek P, Nellaker C, McIntyre R, Buendia-Buendia J, Bumpstead S, Ponting C, et al. High levels of RNA-editing site conservation amongst 15 laboratory mouse strains. Genome Biol. 2012;13:r26.View ArticlePubMed CentralGoogle Scholar
- Ramaswami G, Zhang R, Piskol R, Keegan LP, Deng P, O’Connell MA, et al. Identifying RNA editing sites using RNA sequencing data alone. Nat Methods. 2013;10:128–32.View ArticlePubMedPubMed CentralGoogle Scholar
- 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.View ArticlePubMedPubMed CentralGoogle Scholar
- 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.View ArticlePubMedPubMed CentralGoogle Scholar
- 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.View ArticlePubMedGoogle Scholar
- Peisley A, Jo MH, Lin C, Wu B, Orme-Johnson M, Walz T, et al. Kinetic mechanism for viral dsRNA length discrimination by MDA5 filaments. Proc Natl Acad Sci U S A. 2012;109:E3340–3349.View ArticlePubMedPubMed CentralGoogle Scholar
- Ota H, Sakurai M, Gupta R, Valente L, Wulff BE, Ariyoshi K, et al. ADAR1 forms a complex with Dicer to promote microRNA processing and RNA-induced gene silencing. Cell. 2013;153:575–89.View ArticlePubMedPubMed CentralGoogle Scholar
- Zipeto MA, Court AC, Sadarangani A, Delos Santos NP, Balaian L, Chun HJ, et al. ADAR1 activation drives leukemia stem cell self-renewal by impairing Let-7 biogenesis. Cell Stem Cell. 2016;19:177–91.View ArticlePubMedPubMed CentralGoogle Scholar
- Chen T, Xiang JF, Zhu S, Chen S, Yin QF, Zhang XO, et al. ADAR1 is required for differentiation and neural induction by regulating microRNA processing in a catalytically independent manner. Cell Res. 2015;25:459–76.View ArticlePubMedPubMed CentralGoogle Scholar
- Bahn JH, Ahn J, Lin X, Zhang Q, Lee JH, Civelek M, et al. Genomic analysis of ADAR1 binding and its involvement in multiple RNA processing pathways. Nat Commun. 2015;6:6355.View ArticlePubMedPubMed CentralGoogle Scholar
- Yang W, Chendrimada TP, Wang Q, Higuchi M, Seeburg PH, Shiekhattar R, et al. Modulation of microRNA processing and expression through RNA editing by ADAR deaminases. Nat Struct Mol Biol. 2006;13:13–21.View ArticlePubMedGoogle Scholar
- Kawahara Y, Zinshteyn B, Sethupathy P, Iizasa H, Hatzigeorgiou AG, Nishikura K. Redirection of silencing targets by adenosine-to-inosine editing of miRNAs. Science. 2007;315:1137–40.View ArticlePubMedPubMed CentralGoogle Scholar
- Stellos K, Gatsiou A, Stamatelopoulos K, Perisic Matic L, John D, Lunella FF, et al. Adenosine-to-inosine RNA editing controls cathepsin S expression in atherosclerosis by enabling HuR-mediated post-transcriptional regulation. Nat Med. 2016;22:1140–50.View ArticlePubMedGoogle Scholar
- Wang Q, Hui H, Guo Z, Zhang W, Hu Y, He T, et al. ADAR1 regulates ARHGAP26 gene expression through RNA editing by disrupting miR-30b-3p and miR-573 binding. RNA. 2013;19:1525–36.View ArticlePubMedPubMed CentralGoogle Scholar
- Rueter SM, Dawson TR, Emeson RB. Regulation of alternative splicing by RNA editing. Nature. 1999;399:75–80.View ArticlePubMedGoogle Scholar
- Schoft VK, Schopoff S, Jantsch MF. Regulation of glutamate receptor B pre-mRNA splicing by RNA editing. Nucleic Acids Res. 2007;35:3723–32.View ArticlePubMedPubMed CentralGoogle Scholar
- Feng S, Li H, Zhao J, Pervushin K, Lowenhaupt K, Schwartz TU, et al. Alternate rRNA secondary structures as regulators of translation. Nat Struct Mol Biol. 2011;18:169–76.View ArticlePubMedGoogle Scholar
- Storer JB. Longevity and gross pathology at death in 22 inbred mouse strains. J Gerontol. 1966;21:404–9.View ArticlePubMedGoogle Scholar
- Kunstyr I, Leuenberger HG. Gerontological data of C57BL/6 J mice. I. Sex differences in survival curves. J Gerontol. 1975;30:157–62.View ArticlePubMedGoogle Scholar
- Snyder EM, Licht K, Braun RE. Testicular adenosine to inosine RNA editing in the mouse is mediated by ADARB1. Biol Reprod. 2017;96:244–53.PubMedGoogle Scholar
- Wang GG, Calvo KR, Pasillas MP, Sykes DB, Hacker H, Kamps MP. Quantitative production of macrophages or neutrophils ex vivo using conditional Hoxb8. Nat Methods. 2006;3:287–93.View ArticlePubMedGoogle Scholar
- Ward SV, George CX, Welch MJ, Liou LY, Hahm B, Lewicki H, et al. RNA editing enzyme adenosine deaminase is a restriction factor for controlling measles virus replication that also is required for embryogenesis. Proc Natl Acad Sci U S A. 2011;108:331–6.View ArticlePubMedGoogle Scholar
- Yu S, Sharma R, Nie D, Jiao H, Im HJ, Lai Y, et al. ADAR1 ablation decreases bone mass by impairing osteoblast function in mice. Gene. 2013;513:101–10.View ArticlePubMedGoogle Scholar
- Ng AJ, Walia MK, Smeets MF, Mutsaers AJ, Sims NA, Purton LE, et al. The DNA helicase Recql4 is required for normal osteoblast expansion and osteosarcoma formation. PLoS Genet. 2015;11:e1005160.View ArticlePubMedPubMed CentralGoogle Scholar
- Zhang R, Li X, Ramaswami G, Smith KS, Turecki G, Montgomery SB, et al. Quantifying RNA allelic ratios by microfluidic multiplex PCR and sequencing. Nat Methods. 2014;11:51–4.View ArticlePubMedGoogle Scholar
- Pinto Y, Cohen HY, Levanon EY. Mammalian conserved ADAR targets comprise only a small fragment of the human editosome. Genome Biol. 2014;15:R5.View ArticlePubMedPubMed CentralGoogle Scholar
- Riedmann EM, Schopoff S, Hartner JC, Jantsch MF. Specificity of ADAR-mediated RNA editing in newly identified targets. RNA. 2008;14:1110–8.View ArticlePubMedPubMed CentralGoogle Scholar
- Essers MA, Offner S, Blanco-Bose WE, Waibler Z, Kalinke U, Duchosal MA, et al. IFNalpha activates dormant haematopoietic stem cells in vivo. Nature. 2009;458:904–8.View ArticlePubMedGoogle Scholar
- Crow YJ, Manel N. Aicardi-Goutieres syndrome and the type I interferonopathies. Nat Rev Immunol. 2015;15:429–40.View ArticlePubMedGoogle Scholar
- Han L, Diao L, Yu S, Xu X, Li J, Zhang R, et al. The genomic landscape and clinical relevance of A-to-I RNA editing in human cancers. Cancer Cell. 2015;28:515–28.View ArticlePubMedPubMed CentralGoogle Scholar
- Chen L, Li Y, Lin CH, Chan TH, Chow RK, Song Y, et al. Recoding RNA editing of AZIN1 predisposes to hepatocellular carcinoma. Nat Med. 2013;19:209–16.View ArticlePubMedPubMed CentralGoogle Scholar
- Heraud-Farlow JE, Walkley CR. The role of RNA editing by ADAR1 in prevention of innate immune sensing of self-RNA. J Mol Med (Berl). 2016;94:1095–102.View ArticleGoogle Scholar
- Daniel C, Lagergren J, Ohman M. RNA editing of non-coding RNA and its role in gene regulation. Biochimie. 2015;117:22–7.View ArticlePubMedGoogle Scholar
- Levanon EY, Eisenberg E. Does RNA editing compensate for Alu invasion of the primate genome? Bioessays. 2015;37:175–81.View ArticlePubMedGoogle Scholar
- Yao H, Dittmann M, Peisley A, Hoffmann HH, Gilmore RH, Schmidt T, et al. ATP-dependent effector-like functions of RIG-I-like receptors. Mol Cell. 2015;58:541–8.View ArticlePubMedPubMed CentralGoogle Scholar
- Volkman HE, Stetson DB. The enemy within: endogenous retroelements and autoimmune disease. Nat Immunol. 2014;15:415–22.View ArticlePubMedPubMed CentralGoogle Scholar
- Washburn MC, Kakaradov B, Sundararaman B, Wheeler E, Hoon S, Yeo GW, et al. The dsRBP and inactive editor ADR-1 utilizes dsRNA binding to regulate A-to-I RNA editing across the C. elegans transcriptome. Cell Rep. 2014;6:599–607.View ArticlePubMedPubMed CentralGoogle Scholar
- Li Y, Banerjee S, Goldstein SA, Dong B, Gaughan C, Rath S, et al. Ribonuclease L mediates the cell-lethal phenotype of double-stranded RNA editing enzyme ADAR1 deficiency in a human cell line. Elife. 2017;6:e25687.PubMedPubMed CentralGoogle Scholar
- Gitlin L, Barchet W, Gilfillan S, Cella M, Beutler B, Flavell RA, et al. Essential role of mda-5 in type I IFN responses to polyriboinosinic:polyribocytidylic acid and encephalomyocarditis picornavirus. Proc Natl Acad Sci U S A. 2006;103:8459–64.View ArticlePubMedPubMed CentralGoogle Scholar
- Ventura A, Kirsch DG, McLaughlin ME, Tuveson DA, Grimm J, Lintault L, et al. Restoration of p53 function leads to tumour regression in vivo. Nature. 2007;445:661–5.View ArticlePubMedGoogle Scholar
- Smeets MF, DeLuca E, Wall M, Quach JM, Chalk AM, Deans AJ, et al. The Rothmund-Thomson syndrome helicase RECQL4 is essential for hematopoiesis. J Clin Invest. 2014;124:3551–65.View ArticlePubMedPubMed CentralGoogle Scholar
- Hardwick SA, Chen WY, Wong T, Deveson IW, Blackburn J, Andersen SB, et al. Spliced synthetic genes as internal controls in RNA sequencing experiments. Nat Methods. 2016;13:792–8.View ArticlePubMedGoogle Scholar
- Dobin A, Davis CA, Schlesinger F, Drenkow J, Zaleski C, Jha S, et al. STAR: ultrafast universal RNA-seq aligner. Bioinformatics. 2013;29:15–21.View ArticlePubMedGoogle Scholar
- Robinson MD, McCarthy DJ, Smyth GK. edgeR: a Bioconductor package for differential expression analysis of digital gene expression data. Bioinformatics. 2010;26:139–40.View ArticlePubMedGoogle Scholar
- Mi H, Huang X, Muruganujan A, Tang H, Mills C, Kang D, et al. PANTHER version 11: expanded annotation data from Gene Ontology and Reactome pathways, and data analysis tool enhancements. Nucleic Acids Res. 2017;45:D183–9.View ArticlePubMedGoogle Scholar
- Yaari G, Bolen CR, Thakar J, Kleinstein SH. Quantitative set analysis for gene expression: a method to quantify gene set differential expression including gene-gene correlations. Nucleic Acids Res. 2013;41:e170.View ArticlePubMedPubMed CentralGoogle Scholar