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Many large noncoding RNAs (lncRNAs) regulate chromatin, but the mechanisms by which they localize to genomic targets remain unexplored. Here we investigate the localization mechanisms of the Xist lncRNA during X-chromosome inactivation (XCI), a paradigm of lncRNA-mediated chromatin regulation. During the maintenance of XCI, Xist binds broadly across the X-chromosome. During initiation of XCI, Xist initially transfers to distal regions across the X-chromosome that are not defined by specific sequences. Instead, Xist identifies these regions by exploiting the three-dimensional conformation of the X-chromosome. Xist requires its silencing domain to spread across actively transcribed regions and thereby access the entire chromosome. This suggests a model where Xist coats the X-chromosome by searching in three dimensions, modifying chromosome structure, and spreading to newly accessible locations.
Mammalian genomes encode thousands of large non-coding RNAs (lncRNAs) (1-5), many of which play key functional roles in the cell (6-9). One emerging paradigm is that many lncRNAs can regulate gene expression (6, 8-11) by interacting with chromatin regulatory complexes (6, 12-14) and localizing these complexes to genomic target sites (15-17). Despite the central role of RNA-chromatin interactions, the mechanisms by which lncRNAs identify their genomic targets remain unexplored.
The Xist ncRNA provides a model to investigate the mechanisms of lncRNA localization (11, 18, 19). Xist initiates X-chromosome inactivation (XCI) by spreading in cis across the future inactive X-chromosome (20, 21), recruiting the polycomb repressive complex 2 (PRC2) (14, 22, 23), and forming a transcriptionally silent nuclear compartment (24, 25) enriched for repressive chromatin modifications including H3K27me3 (22, 23). These functions of Xist – localization to chromatin and silencing of gene expression – are mediated by distinct RNA domains (26): transcriptional silencing requires the A-repeat domain (26), which interacts with the PRC2 chromatin regulatory complex (14), while localization to chromatin requires several distinct domains (26-28) and interactions with proteins associated with the nuclear matrix (29-31). Despite these advances in our understanding of Xist, we still do not understand the process by which Xist localizes to chromatin and spreads across the X-chromosome.
Here we present a biochemical method that enables high-resolution mapping of lncRNA localization. Using this method, we explored Xist localization during initiation and maintenance of XCI. During maintenance, Xist localized broadly across the entire X-chromosome, lacking focal binding sites. During initiation of XCI, Xist transferred directly from its transcription locus to distal sites across the X-chromosome that are defined not by specific sequences but by their spatial proximity in the nucleus to the Xist transcription locus. Furthermore, we show that Xist initially localized to the periphery of actively transcribed regions, but gradually spread across them through a mechanism dependent on the A-repeat domain. Together, these results suggest that Xist initially localizes to distal sites across the chromosome by exploiting chromosome conformation, and may spread to new sites through its ability to modify chromatin structure.
To determine the genomic localization of lncRNAs, we developed a method termed RNA Antisense Purification (RAP), which is conceptually similar to previous methods (32-34) in that it uses biotinylated antisense probes that hybridize to a target RNA to purify the endogenous RNA and its associated genomic DNA from crosslinked cell lysate (Fig. 1A) (35). We designed RAP to enable specific purification of chromatin associated with a target lncRNA, achieve high resolution mapping of the associated DNA target sites upon sequencing of the captured DNA, and robustly capture any lncRNA with minimal optimization. To achieve high specificity, RAP utilizes 120-nucleotide antisense RNA probes in order to form extremely strong hybrids with the target RNA thereby enabling purification using denaturing conditions that disrupt nonspecific RNA-protein interactions and nonspecific hybridization with RNAs or genomic DNA. To achieve high resolution, RAP uses DNase I to digest genomic DNA to ~150bp fragments, which provides high resolution mapping of binding sites. To robustly capture a lncRNA, RAP uses a pool of overlapping probes tiled across the entire length of the target RNA to ensure capture even in the case of extensive protein-RNA interactions, RNA secondary structure, or partial RNA degradation (supplementary online text).
To test our method, we used RAP to purify the Xist RNA and associated DNA from female mouse lung fibroblasts (MLFs), a differentiated cell line in which Xist is expressed from and coats the inactive X-chromosome. We designed antisense probes tiled every 15 nucleotides across the 17-Kb Xist transcript, excluding those that showed any complementarity to other RNAs or genomic DNA regions (35). This yielded a pool of 1,054 unique probes. We performed RAP and observed a >100-fold enrichment of the Xist RNA compared to either input or a control purification using ‘sense’ probes from the same strand as Xist itself (Fig. 1B). When we sequenced all RNAs in the purified fraction, we found that the Xist RNA comprised ~70% of alignable reads despite representing <0.1% of the polyadenylated input RNA. The remaining reads were broadly distributed across ~7,500 expressed transcripts, with no single transcript exceeding 2% of the total purified RNA (Fig. 1C). We sequenced the genomic DNA that co-purified with the Xist RNA and observed a strong enrichment with >70% of the DNA sequencing reads from the Xist purification originating from the X-chromosome, compared to ~5% from the input DNA samples (Fig. 1D).
To ensure that the DNA purified by Xist RAP reflected the endogenous localization of Xist, we performed three controls (Fig. S1) (35). (i) To confirm that captured chromatin reflected pre-existing interactions occurring in vivo, we purified Xist from non-crosslinked cellular extracts. In this condition, we did not obtain any detectable DNA signal by qPCR despite obtaining comparable enrichments of the Xist RNA (35). (ii) To rule out the possibility that RAP captured genomic DNA through nonspecific hybridization with the probes or the target RNA, we tested whether sites with higher enrichment in Xist RAP showed complementarity to sequences present in the probes or Xist RNA sequence (35). We observed no relationship between sequence homology and RNA localization either on the X-chromosome or on autosomes (Fig. S2). (iii) To further exclude the possibility of direct probe-DNA interactions, we examined DNA captured in a control purification with sense probes which should capture double-stranded DNA with the same efficiency, but will not hybridize to the target RNA. Using the sense probes, we observed no enriched regions across the entire genome (Fig. 1D) with the sole exception of a low-level enrichment at the Xist locus itself (35), likely reflecting perfect hybridization with the RNA probes. Yet, the amount of Xist genomic DNA purified in the control was <5% of the amount in the Xist purification, suggesting that most of the signal in Xist RAP resulted from RNA-mediated interactions (supplemental online text).
Together, these results demonstrate the specificity of the RAP method to capture RNA interactions with chromatin.
Using RAP, we explored the localization of Xist in MLFs. We found that Xist showed enrichment over the entire X-chromosome as opposed to showing punctate enrichment at specific locations (Fig. 2A-C, Fig. S3). Indeed, >95% of 10-Kb windows on the X-chromosome were enriched more than 10-fold compared to the input. In comparison, not a single window on an autosome reached this enrichment level (Fig. 2C). This broad localization pattern contrasts sharply with the roX2 ncRNA in Drosophila, which, despite its similar function of regulating gene expression across an entire chromosome, binds at discrete sites (32, 33).
While Xist showed enrichment across the entire X-chromosome (average enrichment = 23-fold), we observed differences in the precise levels of enrichment across the chromosome (Fig. 2A), which were highly reproducible between replicates (Pearson's correlation = 0.94, Fig. S4) (35). To characterize this variation, we correlated Xist enrichment with other genomic features (Table S1). We found that Xist enrichment strongly correlated with H3K27me3 across the entire chromosome (Pearson's correlation = 0.69, Fig. 2A-B), consistent with the known role for Xist in the recruitment of PRC2 (14, 22, 23). Xist levels also showed a strong correlation with gene density (Pearson's correlation = 0.44) and a negative correlation with the density of LINE repeats (Pearson's correlation = −0.25) which tend to reside in gene-poor regions.
To further explore this variation, we examined the most-enriched (>30-fold) and least-enriched (<15-fold) regions of the X-chromosome (Fig. 2C) (35). The most-enriched regions show higher H3K27me3 occupancy in MLFs (1.7-fold) and higher gene density (3-fold) than the chromosome average, consistent with the chromosome-wide correlations. The least enriched regions contained genes known to escape XCI (36). Consistent with their preferential positioning outside of the Xist domain (37, 38), escape genes displayed a ~50% reduction in Xist occupancy compared to silenced X-chromosome genes, with the level of Xist enrichment roughly reflecting the previously reported ratio of expression from the inactive versus active X-chromosome (Pearson correlation = −0.66, Fig. 2D) (35)(39). Closer examination of Xist localization at some escape genes sometimes revealed sharp boundaries separating escaped and non-escaped domains (Fig. 2E). One of the least-enriched regions resided immediately distal to the Xist locus and included the lncRNA genes Jpx and Ftx, both of which have been previously reported to escape XCI and act as positive regulators of Xist(40, 41) (Fig. 2F).
Altogether, the least-enriched regions contain 53 genes with more than 40% depletion for Xist compared to the chromosome average (Table S2). Twenty-four of these genes have been previously reported to partially escape inactivation, including ten microRNA genes (42) and three lncRNAs (Table S2). Three of these genes represent novel candidate escape genes in MLF, displaying on average 50% depletion of Xist compared to other genes on the X-chromosome. The remaining genes are not expressed in MLF or are located within 300-Kb of a known escape gene and thus likely do not escape XCI in this cell type.
Thus, the Xist RNA localizes broadly across the entire inactive X-chromosome in differentiated cells, preferentially localizing at gene-rich regions (43, 44) but excluding genes that are expressed on the inactive X-chromosome. This broad localization pattern suggests that Xist localizes to chromatin in a degenerate fashion, possibly through interactions with the nuclear matrix (29, 30, 44).
To gain insights into how Xist establishes this broad localization pattern during the initiation of XCI, we examined Xist localization upon activation in mouse embryonic stem (ES) cells (20). In the pluripotent state, Xist is not expressed and both X-chromosomes are active (20, 21, 45, 46). Induction of differentiation triggers Xist activation on one allele, leading to the silencing of the X-chromosome in cis(20, 21, 45). To synchronize the initiation of XCI, we engineered a tetracycline-inducible promoter to drive Xist expression from its endogenous locus in a male mouse ES cell line (Fig. 3A, Fig. S5) (35). Upon induction with doxycycline, these cells increased Xist expression ~120-fold over a period of six hours (Fig. S6). RNA FISH showed that after one hour of induction Xist appeared as a strong focal point and grew to a characteristic cloud over time (Fig. 3B, Fig. S6), accompanied by exclusion of RNA polymerase II and accumulation of PRC2 and H3K27me3 over the Xist RNA compartment (Fig. S6). Cells expressing Xist concurrently silenced expression of the Tsix RNA, which negatively regulates Xist in ES cells (Fig. S6) (47).
To observe the process by which Xist initially spreads across the X-chromosome, we used RAP to generate high-resolution maps of Xist localization across 5 time points between zero and six hours after Xist induction (Fig. 3C, Fig. S7). After one hour of Xist induction, we observed a strong ~5-Mb peak centered at the Xist transcription locus, corresponding to the spot of Xist localization observed using RNA FISH (Fig. 3B, Fig. S6). Over the time-course, this peak declined while Xist levels across the chromosome increased. These patterns mirrored the emergence of the large Xist cloud observable by FISH at these time points. By six hours, the pattern of Xist localization began to resemble stable XCI in MLFs, where Xist localizes broadly across the X-chromosome and is preferentially enriched at gene-dense regions (Fig. S7).
Two models have been proposed to explain how Xist accomplishes this rapid spreading across the entire X-chromosome (Fig. 3D) (44, 48): either Xist spreads uniformly from its transcription site until it coats the entire chromosome, or Xist first localizes to “early” sites that are far from the Xist transcription locus (44). To distinguish between these models, we examined Xist localization by RAP after one hour of Xist induction. We identified 28 distal sites of Xist occupancy across the chromosome (P < 0.05, Fig. 3E) (35). These sites comprised broad domains (average size 367 Kb) that were concentrated in 15 regions spaced across the entire X-chromosome. These sites initially showed an ~2-fold enrichment compared to neighboring regions, but this enrichment decreased over time (Fig. 3C), suggesting that Xist preferentially localizes to these sites early during the initiation of XCI. We also performed the RAP experiment across a differentiation time-course in wild-type female ES cells (Fig. S8) (35). We found that Xist localized to these same distal sites across the X-chromosome in female ES cells (Fig. 3F, Fig. S7, Fig. S9), demonstrating that Xist also targets these early sites in a normal developmental context. Thus, Xist initially transfers from its transcription locus to distal early localization sites to initiate spreading across the X-chromosome.
To determine how Xist identifies and targets these early localization sites, we considered two possible explanations (Fig. 4A). (i) Early sites may have higher affinity for the Xist RNA, enabling them to recruit Xist as it diffuses away from its transcription locus (‘affinity transfer’) (48-51). (ii) Alternatively, early sites may be defined not by affinity for Xist RNA but by spatial proximity to the site of Xist transcription (‘proximity transfer’) (44, 49).
We first explored the affinity transfer model. Early sites were not enriched for specific sequence motifs that could play a role in recruiting Xist (35). We further compared Xist enrichment to >250 genomic annotations, including features such as repeat element density and ChIP-Seq experiments in ES cells (Table S1) (35). We did not observe a significant relationship between Xist localization and LINE1 repeat elements (Pearson's correlation = −0.17) (supplementary online text). Instead, Xist early localization sites displayed modest enrichments (<2-fold) for gene density (Table S3). Yet, the chromosome-wide correlation between Xist localization and gene density was relatively modest (Pearson's correlation = 0.34) (35), suggesting that gene density alone does not explain early Xist localization patterns.
In the proximity transfer model (Fig. 4A) the early Xist localization sites would be in close spatial proximity to the Xist transcription locus prior to Xist RNA induction, allowing direct transfer upon transcription of Xist RNA from its genomic locus to linearly distant chromosomal regions. To test this hypothesis, we examined the conformation of the X-chromosome using a previously published male mouse ES cell dataset (52) generated by genome-wide chromosome conformation capture (Hi-C (53)). Because of the sparseness of the Hi-C contact maps, we binned the data into 1-Mb regions based on the distance from the Xist genomic locus (35). We found a strong correlation between Xist RNA localization across the X-chromosome and the frequency at which distal sites contact the Xist genomic locus (Pearson's correlation = 0.69, Fig. 4B). We note that this correlation is not driven by the strong peak in both datasets centered at the Xist genomic locus because we considered only sites further than 10 Mb from Xist itself (35). This strong correlation was also observed upon differentiation of female ES cells (Pearson's correlation = 0.69, Fig. S10A). These correlations exceeded that of any of the >250 genomic annotations that we tested in ES cells (Table S1).
One possible explanation for this correlation is that RAP might be capturing distal sites due to their proximity-mediated contacts with the Xist DNA locus, rather than due to interactions with the Xist RNA. This is possible because in Xist RAP the Xist DNA locus is enriched ~10-fold compared to the rest of the X-chromosome (Fig. 4B). By capturing the Xist DNA locus through purification of Xist RNA, we might indirectly enrich other distal sites that are crosslinked to the Xist DNA locus, thereby yielding a pattern of enrichment similar to a standard chromosome conformation capture assay. However, if we observed a similar correlation between early Xist localization and chromosome conformation in the absence of a strong localization peak at the Xist genomic locus, then the pattern of Xist enrichment across the chromosome cannot be explained by proximity-induced crosslinking effects. To test this, we used our inducible system to turn off Xist transcription after one hour of induction and profiled Xist localization (35). We found that Xist RNA enrichment at its DNA locus declined from 102-fold to 14-fold over input, showing a level comparable to the rest of the X-chromosome (Fig. S10B). Xist remained enriched at the same distal regions (Fig. S7, Fig. S9) and showed a comparable correlation with proximity contacts to the Xist DNA locus (Pearson's correlation = 0.59, Fig. S10C), arguing that the Xist RNA interacts directly with these spatially proximal sites.
These data demonstrate that early Xist localization correlates with spatial proximity, but do not demonstrate a causal relationship between Xist localization and chromosome conformation. If initial Xist localization is controlled by proximity-mediated contact with the Xist genomic locus, then altering the conformational context of the Xist transcription locus should lead to an early localization pattern defined by the proximity contacts of the new integration site. To test this directly, we utilized a male ES cell line that expresses an Xist cDNA from a Tet-inducible transgene incorporated at the Hprt locus, a genomic locus ~50 Mb proximal to the endogenous Xist locus (26) (Fig. S7, Fig. S10D). When we examined these cells at early time points after induction, we found that early Xist localization correlated strongly with proximity contacts at the Hprt integration site (Pearson's correlation = 0.92, Fig. 4C) but not with those at the endogenous Xist locus (Pearson's correlation = −0.02). While these results do not exclude the possibility that additional chromatin features may be important for creating a permissive environment for Xist RNA localization, it is clear that chromosome conformation plays a dominant role in determining the early localization sites of the Xist RNA on the X-chromosome.
Thus, spatial proximity to the Xist transcription locus guides early Xist RNA localization. This proximity-guided search may explain several of our other observations about Xist localization. (i) Because Xist is actively transcribed, it will be located within the ‘active compartment’ of the nucleus (53). This may explain our observations that Xist preferentially localizes to gene-rich regions. (ii) Because chromosome conformation is heterogeneous in a cell population (54, 55), the precise order by which Xist spreads to distal sites is likely to differ between individual cells. This may explain why Xist shows low-level early enrichment across the entire X-chromosome as all regions of the chromosome may contact the Xist genomic locus at some low frequency.
Although early Xist localization correlated strongly with proximity contact frequency across the chromosome, we noticed several large chromosomal domains where Xist occupancy was lower than would be expected based on the observed proximity contacts (e.g., black arrows in Fig. 4B). These depleted regions contained many genes that are actively transcribed in ES cells; we termed these “active gene-dense regions”. In contrast, the early-enriched Xist localization sites were also gene-dense but were enriched for genes that are inactive in ES cells. The depleted regions neighbored the early Xist localization sites such that Xist accumulated on the periphery of active gene-dense regions (Fig. S11A).
To test whether actively transcribed genes generally showed reduced Xist occupancy, we explored Xist localization across all genes on the X-chromosome three hours after Xist induction. Indeed, Xist showed on average a 15% focal depletion over active genes (P = 0.006, Mann-Whitney test), but was not depleted across inactive genes (Fig. 5A,B). The level of Xist occupancy across active genes roughly reflected the level of expression in ES cells, with highly transcribed genes showing the lowest Xist occupancy (Pearson's correlation = -0.33, Fig. S11B). Furthermore, this focal depletion across active genes was temporary: Xist enrichment at genes expressed in ES cells increased over time and upon stable inactivation in MLFs was comparable to neighboring intergenic regions and inactive genes (Fig. S11C). Together, these results suggest that the initial localization of Xist is hindered by some feature of actively transcribed genes but that Xist can eventually overcome this barrier to spread across these regions.
We hypothesized that the ability of Xist to spread across active genes is dependent on its ability to silence gene expression. Previous genetic studies have identified the A-repeat within Xist as an RNA domain that is necessary for silencing gene expression but that is not required for the formation of the Xist RNA compartment (25, 26). We therefore repeated the RAP experiments using an Xist RNA in which the A-repeat had been deleted (ΔA Xist) (26). We found that the localization of ΔA Xist over the whole X-chromosome looked broadly comparable to that of wild-type Xist (Fig. 5C, Fig. S12), consistent with previous observations by FISH (25, 26). However, at high resolution, we observed a ~2-fold depletion for ΔA Xist occupancy compared to wild-type Xist over active gene-dense regions, with ΔA Xist instead accumulating on the edges of these regions (Fig. 5C, Fig. S11D,E). This depletion extended across the entire region including active and inactive genes as well as intergenic sequences, suggesting that active gene-dense regions may loop out of the ΔA Xist compartment such that even inactive genes remain physically inaccessible to ΔA Xist spreading (Fig. 5E).
These results demonstrate that Xist initially localizes to the periphery of active gene-dense regions through a mechanism independent of its A-repeat domain, but requires the A-repeat to efficiently spread across active genes and access these regions. Notably, the A-repeat domain interacts with the PRC2 chromatin-modifying complex (14) and enables the spatial repositioning of active genes into the Xist compartment (25). Together, these observations suggest that the A-repeat may allow Xist to access and spread across active gene-dense regions by modifying chromatin and altering chromosome architecture to reposition these regions into the Xist compartment (Fig. 5E).
Our data suggest a model for how Xist can integrate its two functions – localization to DNA and silencing of gene expression – to exploit and alter nuclear architecture to spread across the X-chromosome (Fig. 6). In this model, at the initiation XCI, Xist exploits the pre-existing three-dimensional conformation of the X-chromosome to search for target sites across the chromosome. Upon encountering a new site, Xist transfers to this region through a mechanism that allows it to localize to any region of the X-chromosome, possibly through its interaction with proteins in the nuclear matrix (29-31). Initially, Xist accumulates at spatially proximal sites on the periphery of active gene-dense regions, positioning itself to silence neighboring genes. Through the A-repeat domain, Xist leads to transcriptional silencing (26) and repositioning of these genes into the growing Xist silenced compartment (25), possibly through recruitment of PRC2 (14) and other proteins (56) that lead to chromosomal compaction (57, 58). By repositioning previously active regions into its growing compartment, Xist effectively pulls new regions of active chromatin closer to the Xist transcription locus, thus allowing Xist RNA to spread to new sites by proximity transfer. Since Xist is actively transcribed throughout XCI, it will remain spatially close to other actively transcribed genes (59) – the precise targets required for propagating Xist-mediated silencing. This process – involving searching in three dimensions, modifying chromatin state and chromosome architecture, and spreading to newly accessible locations – would explain how Xist can silence the entire X-chromosome reproducibly, such that silencing occurs in each cell, despite the fact that chromosome conformation and thus the early Xist localization sites may vary between individual cells in a population.
This coordinated interplay between lncRNA localization and chromosome conformation may have broader implications beyond Xist. Other lncRNAs may similarly take advantage of chromosome conformation to identify target sites in close spatial proximity (9, 17, 60), which could even reside on other chromosomes (61, 62). This search strategy capitalizes on the ability of a lncRNA to act while tethered to its transcription locus (63), in contrast to an mRNA which requires export and translation to carry out its function. Because chromosome conformation is nonrandom, a proximity-guided search strategy might explain how low-abundance lncRNAs can reliably identify their genomic targets. Upon binding these targets, lncRNAs may in turn alter chromosome conformation through their interactions with various chromatin regulatory complexes (15, 16). These alterations would allow localization to and regulation of previously inaccessible chromatin domains, and might even establish local nuclear compartments that contain the co-regulated targets of lncRNA complexes.
We designed a set of 120-nucleotide oligos tiled every 15 nucleotides across the entire Xist RNA sequence, excluding sequences that originated from a repetitive region. We synthesized this pool of oligos using microarray-based DNA synthesis technology and incorporated T7 promoter sequences through PCR. We generated RNA probes by in vitro transcription in the presence biotin-UTP. We crosslinked cells with 2 mM disuccinimidyl glutarate for 45 minutes and 3% formaldehyde for 10 minutes. We lysed cells and digested chromatin to 100-300 bp fragments through a combination of sonication and treatment with TURBO DNase. We diluted the lysate to hybridization conditions containing 3 M guanidine thiocyanate. We precleared lysate preparations by adding streptavidin-coated magnetic beads for 20 minutes at 45°C. Biotin-labeled RNA capture probes were mixed with the heated lysate and incubated at 45°C for 2 hours. We captured the probe-RNA complexes with streptavidin-coated beads and washed six times at 45°C. We eluted captured chromatin complexes and reversed crosslinks by adding Proteinase K to the probe-bead complexes and incubating overnight at 65°C. We generated standard Illumina sequencing libraries and obtained >5 million 25-bp paired-end reads per sample.
For the time-course, we used a male ES cell line in which the wild-type Xist promoter was replaced with a Tet-inducible promoter. For chromosome conformation and A-repeat deletion experiments, we used male ES cell lines carrying a wild-type or ΔA Xist cDNA transgene in the Hprt locus under control of a Tet-inducible promoter. To induce Xist expression, we added doxycycline to a final concentration of 2 μg/mL at a defined time before fixing cells.
Sequencing reads were aligned to the Mus musculus genome (mm9). We calculated enrichment ratios between read counts in the RAP experiment and the input in overlapping windows across the chromosome. To identify early sites in the time-course experiments, we looked for 100-Kb windows with enrichments that exceeded the local mean (P < 0.05). We correlated Xist enrichment across the chromosome with normalized Hi-C interaction counts measured in male mouse ES cells at 1-Mb resolution (52). For Hi-C correlation analysis, we excluded all bins within 10 Mb on either side of the Xist transcription locus, which would otherwise dominate the correlation calculation due to the strong local peaks in both the Hi-C and RAP datasets. To define active and inactive genes, we analyzed RNA-Seq data from embryonic stem cells and defined “active” genes as those expressed with P < 0.001.
Complete materials and methods are available as supplementary material.
We thank Andi Gnirke for initial discussions about the RAP method; Tarjei Mikkelsen for assistance with oligonucleotide synthesis; Manuel Garber and John Rinn for helpful discussions and ideas; Anton Wutz for generously providing Xist transgenic cell lines; Suhas Rao, Neva Cherniavsky, and Erez Lieberman-Aiden for analytical help and discussions; Pam Russell, Moran Cabili, Ezgi Hacisuleyman, and Loyal Goff for critical reading of the manuscript; Leslie Gaffney for assistance with figures; and Sigrid Knemeyer for illustrations. JE is supported by the Fannie and John Hertz Foundation and NDSEG Fellowships. APJ is supported by an NIH post-doctoral fellowship (1F32GM103139-01). This work was funded by an NIH Director's Early Independence Award (DP5OD012190 to MG), NHGRI Center for Excellence for Genomic Sciences (P50HG006193 to MG), NIGMS (P01GM099134 to KP), CIRM (RN1-00564, RB3-05080, and RB4-06133 to KP), and funds from the Broad Institute of MIT and Harvard (MG and ESL) and the Eli and Edythe Broad Center of Regenerative Medicine and Stem Cell Research at UCLA (KP). JE, ESL, and MG are inventors on a provisional patent on the RAP method. Sequencing data is available online from the NCBI Gene Expression Omnibus (accession GSE46918, http://www.ncbi.nlm.nih.gov/geo/) and additional data and information is available at www.lncRNA.caltech.edu/RAP/.
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