Skeletal muscle satellite cells are quiescent adult resident stem cells that activate, proliferate and differentiate to generate myofibres following injury. They harbour a robust proliferation potential and self-renewing capacity enabling lifelong muscle regeneration. Although several classes of microRNAs were shown to regulate adult myogenesis, systematic examination of stage-specific microRNAs during lineage progression from the quiescent state is lacking. Here we provide a genome-wide assessment of the expression of small RNAs during the quiescence/activation transition and differentiation by RNA-sequencing. We show that the majority of small RNAs present in quiescent, activated and differentiated muscle cells belong to the microRNA class. Furthermore, by comparing expression in distinct cell states, we report a massive and dynamic regulation of microRNAs, both in numbers and amplitude, highlighting their pivotal role in regulation of quiescence, activation and differentiation. We also identify a number of microRNAs with reliable and specific expression in quiescence including several maternally-expressed miRNAs generated at the imprinted Dlk1-Dio3 locus. Unexpectedly, the majority of class-switching miRNAs are associated with the quiescence/activation transition suggesting a poised program that is actively repressed. These data constitute a key resource for functional analyses of miRNAs in skeletal myogenesis, and more broadly, in the regulation of stem cell self-renewal and tissue homeostasis.
Adult skeletal muscles can regenerate robustly to confront mild and severe lesions induced by exercise or trauma. This extraordinary regenerative capacity occurs largely through the mobilization of resident muscle satellite (stem) cells. These cells are quiescent in resting muscle and can activate, proliferate and differentiate to form new muscle fibres1. During lineage progression, a subset of proliferating satellite cells self-renew in their niche by reversibly exiting the cell cycle. Therefore, skeletal myogenesis is a tractable model to study the regulation of quiescence, self-renewal and differentiation.
Micro-RNAs (miRNAs) are ~22-nucleotide long non-coding RNAs that participate in post-transcriptional regulation of gene expression through mRNAs decay or translational repression2. Stem-loop structured pre-miRNAs are excised from primary miRNAs and exported to the cytoplasm. Further excision of the loop of pre-miRNA by Dicer gives rise to miRNA/miRNA* duplexes. Single-strand miRNAs are then loaded within the RNA-Induced Silencing Complex and guide RISC to complementary sequences in 3′UTR of target mRNAs3,4. The miRNA pathway has been shown to play a major role in cell specification and differentiation in many organisms, and also more broadly in organism development, tissue homeostasis. Germ line loss of Dicer is lethal at gastrulation, demonstrating an absolute requirement of miRNAs for mouse development5. Other studies have demonstrated the specific requirement of miRNAs in ES cells and tissue specific stem cells6,7.
A set of miRNAs is associated with differentiation of skeletal muscle cell lines8,9,10. These so-called myomiRs, are induced by the myogenic transcription factors Myod and Myogenin (Myog), and can promote muscle differentiation in vitro. Conditional deletion of Dicer in myogenic progenitors expressing Myod in embryos (MyodCre; Dicerflox) results in muscle hypoplasia and perinatal lethality11 supporting an essential role of miRNAs in muscle development. This role was further dissected during muscle formation and homeostasis and repair in experiments using a Dicer conditional KO allele in conjunction with the satellite cell Cre recombinase driver mouse Pax7-CreERT2. In this case, satellite cells exiting from quiescence underwent apoptosis, thus resulting in failed regeneration after muscle injury12. The initial finding that some miRNAs were expressed in a tissue-specific fashion was confirmed in a study showing that miR-1, miR-122a and miR-124a expression is restricted to striated muscle, liver and brain, respectively13, whereas 30 miRNAs are enriched or specifically expressed in skeletal muscle14. Interestingly, myomiRs appear to have either uniform expression throughout the muscle (miR-1 and miR-133a)15,16, or are enriched in slow-twitch, type I muscles (miR-206, miR-208b and miR-499)17,18. In addition, several candidate miRNAs that regulate the quiescence-activation transition in satellite cells were identified, most notably miR-27b19, miR-48912, miR-3120 and miR-195/49721.
As previous quantitative and differential data obtained using RT-qPCR or miRNA-microarrays were limited to the quantification of known molecules, we performed an unbiased analysis of small-RNA profiles from stem to differentiated cells in adult myogenesis. Our data provide a key resource for functional studies of the involvement of small-RNAs - including miRNAs, in skeletal muscle, and more broadly in the regulation of stem cell self-renewal and tissue homeostasis.
Small RNA profiling during lineage progression of muscle satellite cells
To identify small RNAs expressed during muscle lineage progression, we sequenced small-RNAs from total RNA of quiescent (freshly isolated), activated (60 h in culture) and differentiated (7 days in culture) myogenic cells. Quiescent satellite cells were isolated by fluorescence-activated cell sorting (FACS) from adult transgenic Tg:Pax7-nGFP22 mouse limb muscles and subsequently lysed for RNA extraction or in vitro culture (Fig. 1A). Immunological staining confirmed that freshly isolated cells expressed Pax7 whereas Myod expression was undetectable (Fig. 1B). Sixty hours after plating in proliferation medium, myoblasts expressed Myod and retained Pax7 expression, whereas the latter was largely lost after 7 days in culture when the majority of the cells differentiated.
After RNA extraction, small RNAs were size-selected on gel (15–35 nucleotides), cloned and sequenced on a Illumina GAIIx platform. For each time point, 2 to 3 biological replicates yielded on average 3.8 million reads [2.3–4.4] that were mapped to Mm9 genome (Fig. 1C). Further alignment of reads to tRNA and mRNA sequences revealed a low level of contamination from degraded tRNA sequences (0.6 to 3%), whereas mRNA sequences were barely detectable, thereby confirming the quality of the samples. As expected, alignment against mature miRNA sequences (miRBase Release 19) highlighted the fact that the vast majority of sequences corresponded to miRNAs (93% [86–97%]) and marginally to intronic sequences (3% [0.6–6%]). Interestingly, myomiRs represented only 3% of miRNAs expressed in quiescent satellite cells, but as high as 74% of miRNAs expressed in differentiated cells (Supplementary Fig. S1A). Other classes of small RNAs and in particular piRNAs were not detected in our samples. We subsequently focused on the expression profiles of miRNAs.
miRNAs are widely expressed throughout the muscle lineage
Following more detailed examination of the miRNA expression data, we observed that out of the 1,281 miRNA sequences used as reference for alignment at the time of the analysis (miRbase r19), 412 (32%) mature miRNAs with an average of more than 10 reads were detected in one biological condition, demonstrating a wide miRNA repertoire expressed in the adult muscle lineage (Fig. 1D). Furthermore, a very large expression range was observed among these miRNAs, with more than 100 miRNAs showing more than 1000 reads in one condition (Fig. 1E). The distribution of the number of expressed miRNAs according to their expression level was closely comparable for each of the quiescent, activated and differentiated biological states, suggesting an overall similar miRNA abundance during myogenic commitment. However, examination of the relative abundance of the few miRNAs highly expressed during quiescence in the other two conditions pointed to dramatic changes in expression of distinct miRNAs (Supplementary Fig. S1B). This observation underscored the importance of robust normalization of the datasets to avoid skewing of the expression profiles as a result of the high expression of a limited number of miRNAs.
miRNAs expression profiles show dynamic regulation during lineage progression
Following normalization, hierarchical clustering regrouped the samples according to each biological condition (Pearson correlation coefficient R2 > 0.92 among replicates) demonstrating the robustness of the datasets (Supplementary Fig. S1C, and Supplementary Table S1). We confirmed the increase in expression of myomiRs (i.e. miR-1, miR-133, miR-206 and miR-378) during myogenic commitment (Supplementary Fig. S2A–E), as well as the expression of quiescence associated miR-195 and miR-489 previously reported (Supplementary Fig. S2F–G)8,10,12,21. However, we did not recapitulate the expression profiles of miR-27b and miR-31 that were reported to be upregulated in Pax3-positive quiescent satellite cells isolated from abdominal and diaphragm muscles (Supplementary Fig. S2H–I)19,20. Our data are in agreement with expression profiles previously published for these miRNAs using RT-qPCR of quiescent and activated satellite cells from limb muscles12.
We then conducted a differential analysis between quiescent satellite cells, activated and differentiated myogenic cells. Out of the 412 miRNAs that were expressed, we identified 249 differentially expressed miRNAs in the 3-pairwise comparisons (corrected p-value < 0.001): 209 between quiescent and activated, 126 between quiescent and differentiated, and 110 between activated and differentiated muscle cells (Fig. 2A–C). Thus, dynamically expressed micro-RNAs appear to be involved in the regulation of each of the tested cell states. Importantly, we observed that the majority of differential miRNA expression patterns were related to the transition from quiescence to activation (Supplementary Fig. S3).
We then grouped the differentially expressed miRNAs according to their expression profiles using K-means clustering which reveals 4 classes (Fig. 2D and Supplementary Table S2). The first consisted of 59 miRNAs whose expression was found to be associated specifically with quiescence. The second and third clusters comprised miRNAs either expressed during activation, or conversely silenced in this cell state; they represented 70 and 64 miRNAs, respectively. Finally, the last cluster was composed of miRNAs showing an increase in expression during commitment and differentiation, among which were the myomiR class. Overall, the most important transition was between quiescence and activation, where more than half of the differentially expressed miRNAs identified were specific to these states. This finding highlights the concerted role that miRNAs play during the regulation in this transition.
Dynamic regulation of miRNAs during regenerative myogenesis in vivo
To validate the expression of differentially regulated miRNAs during commitment in vitro, we isolated myogenic cells from (i) resting Tibialis anterior (TA) muscle, (ii) 3 days post-notexin (snake venom promotes myofibre lysis)23 injury of TA muscle, and (iii) dissociated Extensor digitorium longus (EDL) muscle fibres with stripped satellite cells. To compare the miRNA expression profiles by RT-qPCR across distinct cell states during myogenic commitment, we chose to normalize to the number of cells. Of the 6 differentially expressed miRNAs identified by sequencing that we validated, 5 showed both the expected trend and magnitude of dynamic expression (Fig. 3). For the remaining miRNA (miR-26b), the trend was similar but a less pronounced magnitude was observed. Additionally, we compared our sequencing dataset to the published profiling of miRNAs during in vivo activation obtained by RT-qPCR12. When focusing on the 228 miRNAs that were detected by both methods, we observed an overall concordance of data (Supplementary Fig. S4A). However, a number of miRNAs absent from the RT-qPCR dataset were detected, thereby complementing the miRNA profiles associated with the Quiescence/Activation transition states. Also, several miRNAs amplified by PCR were unambiguously absent from the sequencing dataset (Supplementary Fig. S4B). Taken together, these observations validated our in vitro model of satellite cell lineage progression and the quiescence/activation transition.
A subset of miRNAs is disproportionally upregulated in quiescent satellite cells
Quiescent satellite cells have a reduced cytoplasmic to nuclear ratio, reduced metabolism, and lower levels of total mRNA and protein compared to activated and differentiated cells24,25. Previous reports stated that miRNAs were globally downregulated in human muscle stem cells26. We thus compared the miRNA and total RNA content in quiescent and activated satellite cells and found that the miRNA/total RNA ratio was in the same order of magnitude (T-test, p-value = 0.53; Supplementary Table S3). Moreover, given the per-cell normalization we used in our RT-qPCR assay, our analysis leads us to propose that tens of miRNAs have higher levels of expression in quiescent vs. activated satellite cells. Taken together, these findings suggest that the miRNAs over-expressed during quiescence are potent regulators that exert their effect in satellite cells.
Comparative analysis of expressed miRNAs and Quiescence vs. Activated transcriptomes
Having identified a set of miRNAs specifically expressed during quiescence, we set out to assess their influence globally on the transcriptome by retrieving miRNA targets from Targetscan 7 database (http://www.targetscan.org)27. We selected mRNA targeted of the 123 miRNAs expressed in quiescent, but not in activated satellite cells, and obtained a list of 18,812 transcripts. We then compared their expression levels in quiescent vs. in vivo-activated satellite cells following an injury in 3 published datasets from 3 different laboratories28,29,30. Despite the lab-to-lab heterogeneity that could be observed in these theoretically identical datasets30, we found a significant down-regulation in quiescence of the targeted transcripts (Supplementary Fig. S5). Gene ontology (GO) enrichment analysis of the targets was however not informative due to the very high number of targets identified. We thus reduced this list to the target mRNA identified by applying more stringent criteria on putative targets from Targetscan with at least 1 conserved target site, and a Cumulative weighted context++ score <−0.2 (yielding to 4,814 putative targets), and conserved only those identified by 2 additional prediction tools (TarBase31 and miRDB)32. Once again, this set of 1,172 transcripts showed an overall downregulation in quiescent satellite cells (Supplementary Fig. S5). Given the high number of genes used, we filtered the results from the GO enrichment analysis (FDR <0.001 & enrichment >4). Surprisingly, most functions related to cardiac development regulation were identified in the dataset (Supplementary Table S4). Nevertheless, we also identified functions related to skeletal muscle tissue development (p-value < 5.9E-9), regulation of ubiquitin-protein transferase activity (p-value < 6.6E-4) and somatic stem cell division (p-value < 1.1E-4).
A cluster of microRNAs on chromosome 12 is over-expressed in quiescent satellite cells
A closer examination of the list of differentially expressed miRNAs identified tens of candidates that were located on chromosome 12 and belonged to two large clusters comprised in the Dlk1-Dio3 locus (Fig. 4A). Notably, we found 5 and 25 miRNAs highly expressed in quiescence and lost upon activation of satellite cells from the miR-127/miR-136 and miR-379/miR-410 clusters, respectively (Fig. 4B). This locus is of major importance for the regulation of skeletal muscle hypertrophy33. Additionally, it was reported recently that the deletion of the miR-379/544 locus induced a hypertrophy of fast-twitch muscles in neonates34. We thus chose to investigate the molecular function of these differentially expressed miRNAs specifically in satellite cells. To do so, we used a mouse model carrying a deletion of the maternally expressed miR-379–410 cluster and Mirg non-coding gene35, to assess the consequences of these miRNAs on homeostasis and regeneration (Fig. 4C). We noted that there was no difference in numbers of Pax7+ satellite cells per fibre in resting EDL muscle of WT and KO mice (Fig. 4D). In addition, following Notexin injury of TA muscle, no overt regeneration phenotype was observed in KO mice (Fig. 4E). Finally, isolated satellite cells from both WT and KO resting muscles did not show any significant differences in their ability to proliferate, commit to myogenesis, differentiate, or self-renew as reserve cells in culture (Fig. 4F, data not shown). These findings raise the possibility that other compensatory miRNAs might act to regulate these transitions.
We then selected two candidate miRNAs with robust expression in quiescence for further analysis: miR-127-3p and miR-379-5p. These miRNAs that belong to the miR-127-3p and miR-379-5p clusters were also validated for their modulation of expression after in vivo activation (Fig. 3E–H). We assessed the potential impact of their expression on cell fate decisions by maintaining their expression level using transfected miR-mimics in satellite cells isolated from resting adult muscles. After 72 h culture of satellite cells, both miRNAs promoted a significant increase in the number of Pax7-expressing cells, whereas Myog-positive differentiating cells were reduced compared to control cells transfected with a scramble mimic (Fig. 4G–H). Following sustained expression of a third mimic miR-126-3p, no significant effect in these assays was noted in spite of the robust and specific expression of this miRNA in quiescent satellite cells and its previously demonstrated role in regulating quiescence in HSC36. These observations confirm the regulatory role of two miRNAs in regulating quiescence and self-renewal. However, the cell-cycle exit and proliferation of satellite cells was not altered by mimic-127 and −379, as measured by EdU incorporation (Fig. 4G–H). Given that Notch signalling is critical for satellite cell maintenance37, we examined the expression of miR-127-3p and miR-379-5p in Rbpj null satellite cells and found no significant alteration in their expression (data not shown). Interestingly, all expressed miRNAs from the Dlk1-Dio3 locus except miR-379 were also reported to be highly expressed in long term HSCs38.
We next set out to assess if the potential targets of these two miRNAs were modulated in quiescent vs. activated satellite cell transcriptomes. Targetscan Db predicted 572 and 1,299 targets for miR-127 and miR-379, respectively. Using the same transcriptome datasets as previously, we found an overall significant downregulation of the targets of quiescent miRNAs targets in quiescent satellite cells in two of them (Fig. 5A). The GO analysis on these target lists did however not yield a functional enrichment. To identify potential relevant targets for the regulation of quiescence, we thus crossed this list of potential targets to the 207 and 542 commonly up- and down-regulated genes identified in our recent analysis of eight transcriptome datasets of quiescent satellite cells30. Focusing on genes down-regulated in quiescence, we propose candidates whose knock-down might be mediating miR-127 and miR-379 control of quiescence and self-renewal, and notably epigenetic regulators (SETD8, CBX5 and HMGA2) as well as adhesion/extracellular matrix genes (CDH2, ITGB6 and CD44), or members of the ubiquitination pathway (UBE2E3, UHRF1, RFWD3, CCNF, SKP2).
In the framework of the present work, we provide the first open platform for analysis of small RNAs expressed during lineage progression of adult muscle stem cells. In this adult tissue stem cell paradigm, we did not observe the expression of piwi-RNAs that were reported to be expressed in germ cells39. However, some reads mapped to intronic regions that could constitute mirtrons and endo-siRNAs. Our data show that small RNAs expressed in the muscle lineage overwhelmingly correspond to microRNAs. Several reports have shed light on the regulation of miRNAs in muscle, but they detected only a limited number of small RNAs using RT-qPCR12 or miRNA microarrays21. The only miR-seq dataset reported did not include an isolated quiescent satellite cell sample, impeding the study of miRNA regulation in the transition states from quiescent to activated muscle stem cells40. Our comparisons with that report pointed to some discrepancies (e.g. absence of increase in miR-206 level during satellite cell activation, or absence of deregulation in miR-489 expression during early injury). However, our dataset was globally concordant with an RT-qPCR based analysis12.
We observed massive deregulation of miRNAs during the quiescence-activation transition in mouse satellite cells. This was unexpected given the low level of regulatory activity and reduced cytoplasmic content of quiescent muscle satellite cells. Instead, the relatively high number of miRNAs enriched during quiescence leads us to propose that cellular quiescence represents a poised state that is actively repressed by class-specific miRNAs. We showed experimentally that many miRNAs have a higher expression in quiescent cells compared to activated satellite cells underscoring the notion that the regulation of the quiescent state is an actively maintained process involving in part a large repertoire of miRNAs. Accordingly, the identification of miR-195/497 and miR-489 as regulators of the quiescence/activation transitions, and Notch signalling as a key mediator of the retention of satellite cells in their niche reinforces this notion12,21,37,41.
Our observations in the mouse are in clear contradiction with a report stating that miRNAs were all downregulated in human quiescent satellite cells which led to the proposal that quiescent cells represent minimal regulatory activity26. These discrepancies could be linked to a low number of miRNAs detected in the human study, that impeded the normalization and robustness of the data, or they might be related to bona fide species-specific differences. Interestingly, Pax7-positive quiescent satellite cells showed miR-27b expression, however miR-31 expression that was reported to be present in Pax3-expressing satellite cells was not expressed in Pax7-expressing satellite cells, thus pointing to potential differences in miRNA regulation between Pax3- and Pax7-expressing cells from trunk and limb, respectively19,20.
In this study, we identified novel miRNA candidates as potential regulators of cell state-specific transitions during myogenic lineage progression, and were interested to identify their influence on mRNA levels by combining several datasets of transcriptomes of quiescent satellite cells28,29. We observed an overall downregulation in quiescence of the several thousand mRNAs putatively targeted by quiescence miRNAs. These observations point to a collective control by miRNAs on the expression of specific mRNAs during these cell transitions. The number of miRNAs expressed in quiescence, and thus the number of potential targets identified complicated the global analysis of their function. Nevertheless, using a restricted list of potential targets generated by combining 3 prediction tools, we found Gene Ontologies associated with regulation of muscle development, including skeletal muscle, but more largely of cardiac development.
Having identified the overexpression of tens of miRNAs from two clusters located in the Dlk1-Dio3 locus in quiescent satellite cells, we investigated the impact of the deletion of the miR-379/410 cluster in vivo. Our observation that this resulted in no overt regeneration phenotype or modulation of cell fates of isolated satellite cells leads us to speculate that other miRNAs have overlapping functions with this cluster. In contrast, functional analysis by sustained expression of two miRNAs from the miR-127 and miR-379 loci resulted in a robust phenotype corresponding to an increase in Pax7 expression and reduced commitment towards differentiation, thereby indicating that these miRNAs promote the stem cell state. These findings suggest that these miRNAs play key roles in regulating satellite cell quiescence in adult resting muscles.
In their in vivo genetic inactivation study of a part of the same miR-379/410 cluster, Gao et al. linked their phenotype to the targeting of Dlk1 expression level by miR-32934. Our results appear to differ from this interpretation given that the phenotype induced by miR-127 and miR-379 overexpression do not correspond to results obtained after conditional deletion of Dlk1 in satellite cells42. Specifically, we did not observe altered proliferation, but instead increased self-renewal and decreased differentiation of satellite cells. The absence of a regeneration phenotype in the miR-379/410 mutant mice could be explained by compensations by other miRNAs expressed in quiescence targeting common targets, or other compensatory mechanisms during development following the germline deletion. The implication of a re-expression of the paternal allele of the miRNA-cluster is however unlikely, as no expression of Mirg, a maternally expressed ncRNAs that overlaps with the miR-379/411 cluster, was detected in satellite cells in mutant mice. Unfortunately, the size of the locus to be deleted precludes the use of a cell type specific inducible Cre-recombinase under the control of Pax7 to study the role of these miRNAs in more detail.
Future work will be required in gain or loss of function experiments to uncover the molecular function of additional differentially expressed miRNAs, and to identify their relevant targets in the context of induction and maintenance of quiescence, beyond the pivotal role of miR-489 and miR-195/497 already noted in Pax7-positive cells. In addition, identifying the signalling pathways upstream of these miRNAs will shed light on this tightly regulated biological process.
In summary, our findings that a relatively significant variety of miRNAs are dedicated to negotiate the quiescence to activation states of muscle stem cells suggests that quiescence is actively repressed by this class of regulators, but in a poised state. These results can impact on our views of genetic and epigenetic regulation of quiescence and how this critical cell state is regulated in homeostasis and trauma.
Mice and flow cytometry of satellite cells
Quiescent muscle stem cells were collected from adult Tg:Pax7-nGFP mice as described previously. Six-weeks old male mice were sacrificed by cervical dislocation, and their limb muscle were dissected, minced and digested in collagenase 0.1% and trypsin 0.25% at 37 °C under gentle agitation. Cells were collected in serum-containing medium and subjected to isolation by FACS based on positive GFP-fluorescence and negative Propidium Iodide fluorescence (10 µg/ml; Sigma-Aldrich). In vivo activated satellite cells were collected by FACS from regenerating injured muscle. The Tibialis anterior (TA) muscles of 6-week-old Tg:Pax7-nGFP mice were injured by intramuscular injection of the snake venom Notexin (10 μl, 10 mM; Latoxan) under anesthesia (0.5% Imalgene/2% Rompun) as described43. Four days after injury, regenerating TA muscles were dissected, dissociated and cells were isolated as aforementioned. Adult limb muscles from miR-379/410 mutant mice were dissected, minced and incubated with a mix of Dispase II (Roche) 3 U/ml, Collagenase A (Roche) 100 ug/ml and DNase I (Roche) 10 mg/ml in Hank’s Balanced Salt Solution (HBSS, Gibco) at 37 °C under gentle agitation for 2 h. Satellite cells were sorted by a combination of cell surface markers: α7-integrin-APC (Ablab, clone R2F2, 1/1000), CD34-e450 (eBioscience, clone RAM34, 1/50), Sca1-Pe-Cy7 (eBioscience, clone D7, 1/400), CD45-Pe-Cy7 (eBioscience, clone 30-F11, 1/100) and CD31-PE (BD, clone MEC13.3, 1/50) as described44,45. All experiments with animals were performed under conditions established by the European Community and approved by the Ethics Committee at Institut Pasteur, and the French Ministry.
Single myofibres from Extensor digitorum longus (EDL) muscle from 6-week-old adult Tg:Pax7-nGFP mice were dissociated as described46. Briefly, EDL muscles were dissected and incubated in 0.1% w/v collagenase (Sigma, C0130)/DMEM for 1 h in a 37 °C shaking water bath. Following mechanical release, individual myofibres were either processed for RNA extraction to validate the RNA sequencing in differentiation conditions, or directly fixed in 4% paraformaldehyde (PFA, Electron Microscopy Sciences).
Satellite cell culture and differentiation
Freshly isolated satellite cells were seeded at 3,000 cells/cm2 in growth medium containing 1:1 DMEM:MCDB (Gibco and Sigma-Aldrich, respectively) supplemented with 20% serum FBS (Gibco) and 1% Ultroser G (Pall) on Matrigel coated flasks (BD Biosciences) and cultured in an incubator under physiological oxygen pressure (37 °C, 6.5% CO2, 3% O2). To assess proliferation, cells were pulsed with the thymidine analogue 5-ethynyl-2′-deoxyuridine (EdU, 1 × 10−6 M), 2 h prior to fixation (ThermoFisher Click-iT Plus EdU kit, C10640). For differentiation experiments, 60 h after plating, medium was replaced to remove Ultroser G, and cells were cultured for a total of 7 days to reach early differentiation.
Satellite cell transfection
Freshly isolated satellite cells from Tg:Pax7-nGFP were transfected in suspension immediately after FACS with miRIDIAN microRNA hsa-miR-126-3p mimic (UCGUACCGUGAGUAAUAAUGCG, Dharmacon, C310987), mmu-miR-379-5p (UGGUAGACUAUGGAACGUAGG, Dharmacon, C310603), mmu-miR-127-3p (UCGGAUCCGUCUGAGCUUGGCU, Dharmacon, C310397) and Scramble Control#1 (UCACAACCUCCUAGAAAGAGUAGA; Dharmacon, CN-001000) at 200 nM final concentration using Lipofectamine 2000 (ThermoFisher) in Opti-MEM (Gibco). Four hours after transfection, 3 volumes of fresh growth medium were added and cells were cultured for the indicated time.
Antibodies and immunostainings
Cells and myofibers were fixed in 4% PFA for 5 min, permeabilised 5 min in 0.5% Triton-X100 (Sigma-Aldrich) and blocked in 10% normal goat-serum (Gibco) for 30 min at RT. Cells and fibres were then incubated with primary antibodies (Chick GFP, Abcam13970,1/2000; mouse Pax7, DHSB, 1/40; rabbit Myod, Santa Cruz, 1/200; mouse Myogenin (F5D), DHSB, 1/40) overnight at 4 °C. Samples were washed with 1X PBS three times and incubated with Alexa-conjugated secondary antibodies (Life Technologies, 1/1000) and Hoechst (Life Technologies, 1/10000) for 45 min at RT. EdU staining was chemically revealed using the Click-iT Plus kit according to manufacturer’s recommendations (Life Technologies, C10640). Images were acquired using an upright fluorescent microscope (Zeiss).
Isolated TA muscles were fixed in PFA 2%/0.2% Triton/PBS 1X for 2 h at 4 °C, washed in PBS 1X overnight at 4 °C and incubated in 20% sucrose/PBS 1X for an additional 12 h. TA muscles were embedded in OCT and frozen in liquid nitrogen prior to cryosectioning (10 µm) and stained with Hematoxylin/Eosin. Images were acquired with Zeiss Axioscan microscope.
Small RNA extraction, deep sequencing and RT-qPCR
For small RNA collection, quiescent cells were directly sorted into Trizol-LS reagent (Invitrogen), and in-vitro cultured cells (activated at 60 hours and differentiated at 7 days) collected in Qiazol reagent (QIagen). Total RNA was subsequently purified using the miRNeasy Mini Kit following the manufacturer's instructions (Qiagen). Ten micrograms of total RNA obtained from several animals for the quiescent samples, were used for each biological replicate prepared for deep sequencing (i.e. 2 replicates for the quiescent and differentiated samples, and 3 replicates for the in vitro activated sample). For RT-qPCR validations all samples were extracted using the same methods (Trizol LS after FACS for quiescent and in-vivo activated satellite cells; Qiazol for isolated single fibres).
For validations, reverse transcription was performed on RNA amount corresponding to fixed absolute number of cells for quiescent and activated SC (i.e. 25,000 cells per RT) in order to be compared. For differentiated muscle fibres, the amount of RNA used in the reverse transcription and following PCR was measured to be equivalent to the activated cells. Reverse transcription of miRNAs was performed on total RNA using the miRCURY LNA Universal RT-PCR system following the manufacturer’s instructions (Exiqon). Quantitative PCR was performed using SYBR Green based mix (Exiqon) and LNA™ PCR primer set (Exiqon) targeting mmu-miR-127-3p (Ref.204048), mmu-miR-379 (Ref.204296), mmu-mir-26a (Ref.204724), mmu-mir-195 (Ref.204186), mmu-miR-183 (Ref.204652), mmu-mir-17 (Ref.204108), U6 snRNA (Ref.203907) and RNU5G (Ref.203908). Analysis was performed using the 2−∆CT method47.
Total mRNA extraction and RT-qPCR
Total mRNAs were isolated using (Qiagen RNAeasy® Micro Kit) and reverse transcribed using SuperScriptIII® enzyme (Invitrogen, 18080093). The remaining RNAs were degraded by incubation for 20 min at 37 °C with RNase H endonuclease (Roche). Expression of mature mRNAs was assessed with SYBR green master mix (Roche) and analyses were performed using the 2−∆∆CT method47. All RT-qPCR analyses were normalized with Tbp and Rpl13. Specific forward and reverse primers used for RT-qPCR are listed in Supplementary Table S5.
Total RNA extraction and Bioanalyser analysis
Total RNAs, including small RNAs, were isolated from quiescent and 48 h in vitro activated satellite cells using Direct-zol RNA Microprep (Zymo Research) according to manufacturer’s recommendations. Total RNA and small RNA ratio were quantified using the Agilent 2100 Bioanalyzer PicoChip and SmallChip and analyzed with 2100 Expert software.
Size fractionation of RNAs
For each biological replicate, 10 µg of total RNA (in 10 µl) were mixed with 10 µl of 2X TBE-Urea Sample Buffer (Invitrogen) and loaded in a well of a 15% polyacrylamide TBE-urea gel (Biorad). After migration, the gel was soaked in a SYBR gold (Invitrogen) solution, and imaged on a Dark Reader transilluminator. The 18–35 nucleotide region was cut using a scalpel for each sample, and the RNA eluted in 300 µl of 0.3 M NaCl solution under rotation for 4 hours at room temperature. The eluate was transferred together with gel debris onto a Spin X cellulose acetate filter (VWR) and centrifuged for 2 minutes at 12,000 xg. Small RNAs were finally precipitated by addition of 1 μl of glycogen (Invitrogen) and 750 μl of room temperature 100% ethanol followed by an incubation at −80 °C for 30 min, and centrifugation for 25 min at 14,000 rpm and + 4 °C. The pellet was washed with 750 µl 75% Ethanol, dried and resuspended in 5 µl ultrapure water with 0.5 µl of RNAseOUT (Invitrogen).
Library preparation for small RNA-seq
Small RNAs purified on gel were mixed to 1 µl of 10 µM pre-adenylated 3′ Illumina linker V1.5 (5′-rAppATCTCGTATGCCGTCTTCTGCTTG/3ddC/-3′), denatured for 2 min at 70 °C, and further mixed with 1 µl of 10x T4 RNA-Ligase Truncated Reaction buffer, 0.8 µl 100 mM MgCl2, 0.5 µl RNaseOut and 1.5 µl of T4 RNA Ligase 2 truncated (New England Biolabs). Ligation was performed at 22 °C for 1 h. Then, 0.5 µl of 5′-RNA adapter (5′-r(GUU CAG AGU UCU ACA GUC CGA CGA UC)-3′), 1 µl of 10 mM ATP and 1 µl T4 RNA ligase (Ambion) were added, and ligation was performed at 20 °C for 6 h. Adaptor ligated RNA in a volume of 4 µl were then mixed with 1 µl of 20 μM Solexa RT primer (5′-CAA GCA GAA GAC GGC ATA CGA-3′) and denatured at 70 °C and cooled on ice. Reverse transcription was then performed after addition of 2 µl 5x first strand buffer (Invitrogen), 0.5 µl of 12.5 mM dNTP mix, 1 µl of 100 mM DTT, 0.5 µl_ RNase OUT and 1 µl SuperScript III Reverse Transcriptase (Invitrogen) at 50 °C for 1 h, followed by 10 min at 70 °C. The obtained cDNA was PCR-amplified by addition of 27 µl Ultra-pure water, 10 µl 5× Phusion-HF buffer, 1 µl of 25 µM Forward Primer (5′-AAT GAT ACG GCG ACC ACC GAC AGG TTC AGA GTT CTA CAG TCC GA-3′), 1 µl of 25 µM reverse Primer (5′-CAA GCA GAA GAC GGC ATA CGA-3′), 0.5 µl of 25 mM dNTP mix, and 0.5 µl Phusion DNA Polymerase (Finnzymes) using 12 cycles 98 °C 10 sec/60 °C 30 sec/72 °C 15 sec. The library was finally purified on a 5% TBE PAGE gel, by cutting the region corresponding to the 92–106 bp (the ligated linkers corresponding to a 73 bp band visible on the gel). The gel was crushed by centrifugation and eluted in 1X Elution buffer (Illumina) by rotation for 2 h at RT. The eluate was cleared using a Spin-X column and precipitated after addition of 1 µl of glycogen, 10 µl of 3 M NaOAc and 325 µl of −20 °C 100% ethanol, followed by centrifugation for 20 min at 14,000 rpm. After washing, the pellet was resuspended in 1 ml dH2O. Finally, the sample was diluted to 10 nM and submitted to sequencing on a Solexa GA-IIX at the core sequencing facility.
Bioinformatic analysis and statistics
Analysis of the microRNAs expression was performed from fastq raw files using the Galaxy Mississipi tool suite (https://mississippi.snv.jussieu.fr) provided by ARTbio bioinformatics analysis facility (Sorbonne Universités, UPMC Univ. Paris 06, CNRS FR3631 Institut de Biologie Paris Seine, Paris, France). Briefly, after trimming of adapters, reads were mapped on Mus musculus mature miRNA sequences from miRbase 19 using sRbowtie. Normalization of miRNAs counts and differential analysis was further performed using DESeq. 2 using replicate samples. MicroRNAs with a corrected p-value < 0.001 (Benjamini-Hochberg method) were considered as differentially expressed. Annotation of reads were performed by sequential alignment of reads on collections of annotated RNA sequences including ribosomal, mitochondrial RNA, exonic and intronic mRNA, piRNA and miRNAs as previously described48.
K-means clustering of differentially expressed miRNAs was performed using Cluster 3.0 (available at bonsai.hgc.jp/~mdehoon/software/cluster/software.htm) using normalized read count as input. After a step of median centering of expression level for each miRNA, clustering was perform using centered Pearson correlation with 1,000 iterations. The corresponding heatmap was generated using JavaTreeView (http://jtreeview.sourceforge.net).
For the mRNA/miRNA correlation analyses, data from Targetscan 7 database were filtered using in-house scripts using stringency in the number of sites and Total context++ score27. For correlation with mRNA expression level, the publicly available datasets GSE47177 and GSE70376 were obtained from the Gene Expression Omnibus (www.ncbi.nlm.nih.gov/geo). Comparisons of expression level between the groups of transcripts in the different satellite cell states (i.e. quiescent or activated in vivo 3 days post injury) were performed using a Mann-Whitney test. All statistical tests were performed in R.
The small RNA-seq data generated and analysed during the current study have been deposited in the ArrayExpress database at EMBL-EBI under accession number E-MTAB-5955 [https://www.ebi.ac.uk/arrayexpress/experiments/E-MTAB-5955].
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We acknowledge the Flow Cytometry Platform of the Technology Core-Center for Translational Science (CRT) and the Transcriptome and EpiGenome Platform of the Center for Innovation & Technological Research at Institut Pasteur for support in conducting this study. S.T. was funded by Institut Pasteur, Centre National pour la Recherche Scientifique and the Agence Nationale de la Recherche (Laboratoire d’Excellence Revive, Investissement d’Avenir; ANR-10-LABX- 73), the European Research Council (Advanced Research Grant 332893) and the French Muscular Dystrophy Association (AFM-Téléthon). M.B.B. was funded by the Fondation pour la Recherche Médicale (FRM). We thank the ABC Facility of ANEXPLO Toulouse for mouse husbandry.
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