Xist RNA expression, methylation of CpG islands, and hypoacetylation of histone H4 are distinguishing features of inactive X chromatin. Here, we show that these silencing mechanisms act synergistically to maintain the inactive state. Xist RNA has been shown to be essential for initiation of X inactivation, but not required for maintenance. We have developed a system in which the reactivation frequency of individual X-linked genes can be assessed quantitatively. Using a conditional mutant Xist allele, we provide direct evidence for that loss of Xist RNA destabilizes the inactive state in somatic cells, leading to an increased reactivation frequency of an X-linked GFP transgene and of the endogenous hypoxanthine phosphoribosyl transferase (Hprt) gene in mouse embryonic fibroblasts. Demethylation of DNA, using 5-azadC or by introducing a mutation in Dnmt1, and inhibition of histone hypoacetylation using trichostatin A further increases reactivation in Xist mutant fibroblasts, indicating a synergistic interaction of X chromosome silencing mechanisms.
In mammals, equal X-linked gene dosage between the sexes is achieved by X chromosome inactivation in females. The inactivated X chromosome resembles constitutive heterochromatin in that it is condensed in interphase (Barr and Carr 1962), hypoacetylated on histone H4 (Jeppesen and Turner 1993), and replicates late in S phase (Priest et al. 1967). It is also methylated on CpG islands of housekeeping genes (Norris et al. 1991) and is enriched in histone macroH2A1, a histone H2A variant with a large nonhistone domain (Costanzi and Pehrson 1998). The inactive X (Xi) expresses Xist (Borsani et al. 1991; Brockdorff et al. 1991; Brown et al. 1991), a nuclear untranslated RNA (Brockdorff et al. 1992) that coats the chromosome in cis (Clemson et al. 1996). Both X chromosomes of an undifferentiated embryonic female cell are active, and X inactivation is initiated at the time of differentiation in vitro or in vivo (Monk and Harper 1979). Once an X chromosome is inactivated in a cell, the inactive state of the chromosome is clonally inherited through many rounds of cell division.
The most remarkable feature of Xi chromatin is its stability with respect to reactivation. Overall experimental reactivation of the entire chromosome in somatic cells has not been observed. Reactivation of one or few genes on the Xi has been seen, but the rate of reactivation is low, on the order of 10−5 to 10−4, in cultured somatic cells (Mohandas et al. 1981; Graves 1982). Many lines of evidence indicate that multiple molecular mechanisms are responsible for the high fidelity of maintenance of X inactivation (for review see Migeon 1994), but the contribution of individual mechanisms to silencing and their complex relationship remains to be elucidated.
Methylation of CpG dinucleotides in the promoter region of repressed genes has long been thought of as a mechanism stabilizing X chromosome inactivation. 5-azadC, an inhibitor of DNA methyltransferase 1 (Dnmt1), the major enzyme responsible for maintaining genomic methylation patterns, has been used to derepress several Xi-linked genes, providing the experimental evidence for the importance of methylation in X inactivation (Mohandas et al. 1981; Graves 1982). Methylation of the CpG island of hypoxanthine phosphoribosyl transferase (Hprt) follows X inactivation by several days, implying that methylation plays a maintenance role (Lock et al. 1987). An in vivo demonstration of the importance of CpG methylation in X inactivation maintenance is the instability of silencing on the Xi of ICF (immunodeficiency centromeric instability facial anomalies) patients. The Xi of patients suffering from ICF syndrome is hypomethylated at all CpG islands analyzed (Hansen et al. 2000). The syndrome is caused by a defect in the DNA methyltransferase DNMT3B (Hansen et al. 1999; Okano et al. 1999; Xu et al. 1999), suggesting that the enzyme may be responsible for establishing CpG methylation on Xi. X inactivation in the virtual absence of CpG methylation is less stable, as evidenced by reactivation of some loci in cells from these patients (Hansen et al. 2000).
Underacetylation of NH2-terminal lysine residues on histones H3 and H4 is another feature of Xi chromatin (Jeppesen and Turner 1993). It is well established that transcriptional activity of genes is regulated by histone acetylation. Histone deacetylation generally correlates with transcriptional silencing and high levels of acetylation with transcriptional activity (Cheung et al. 2000). However, reactivation of X-inactivated genes by altering histone acetylation levels has not been reported. The appearance of a hypoacetylated X chromosome is a late event during differentiation and X inactivation, suggesting that deacetylation of histones is a maintenance rather than establishment mechanism (Keohane et al. 1996).
Xist RNA is essential for the initiation of X chromosome inactivation in cis (Penny et al. 1996; Marahrens et al. 1997). However, several lines of evidence indicate that after X inactivation has been established, Xist is no longer required for maintenance. In studies using mouse–human somatic cell hybrids, a human Xi chromosome fragment that lacked the XIST gene remained transcriptionally silent and its sensitivity to reactivation by 5-azadC did not increase (Brown and Willard 1994). Similarly, in human leukemia cells, an Xi-derived isodicentric chromosome maintained its inactive state despite missing the XIST gene (Rack et al. 1994). To directly address the role of continued Xist RNA expression in karyotypically normal somatic cells, we have previously generated a conditional Xist allele (Csankovszki et al. 1999) using the Cre-loxP system (Sauer and Henderson 1988). After Cre-mediated deletion of Xist in primary mouse embryonic fibroblasts, the Xi remained silent (Csankovszki et al. 1999), again arguing that, in the absence of Xist RNA, other silencing mechanisms are sufficient to keep Xi silent. Another study used embryonic stem cells expressing an inducible Xist cDNA transgene, in which the timing of expression can be experimentally manipulated (Wutz and Jaenisch 2000). This approach defined an initial differentiation time window in which X inactivation is reversible and Xist dependent, followed by irreversible and Xist-independent X inactivation in fully differentiated cells (Wutz and Jaenisch 2000).
Nevertheless, continued transcription of Xist RNA and its close association with Xi throughout the lifetime of the female mammal suggests a role for Xist in somatic cells (Clemson et al. 1996). Indeed, in rodent–human somatic cell hybrids where the human XIST RNA does not localize correctly to Xi (Clemson et al. 1998; Hansen et al. 1998), the stability of silencing is greatly reduced. It has been speculated that reduced efficiency of silencing in hybrid cells is due to the absence of correctly functioning XIST RNA (Clemson et al. 1998; Hansen et al. 1998). Furthermore, deletion of Xist in mouse embryonic fibroblasts disrupts preferential localization of histone macroH2A1 to Xi, and this alteration of chromatin may also lead to decreased stability of silencing (Csankovszki et al. 1999).
To assess the possible role of Xist RNA in X inactivation maintenance and to study the relative contribution of Xist, DNA methylation, and histone hypoacetylation, we developed a system in which even low levels of reactivation can be quantitatively measured. Reactivation of two markers on Xi were studied, a green fluorescent protein (GFP) transgene, GFP (Hadjantonakis et al. 1998), and the endogenous Hprt gene. Using a conditional deletion of Xist (Csankovszki et al. 1999), we provide direct evidence for the first time that Xist RNA contributes to silencing in somatic cells. Additionally, using the drugs 5-azadC and trichostatin A (TSA) and by introducing a mutation in the Dnmt1 gene (Jackson-Grusby et al. 2001), we show that Xist RNA, DNA methylation, and histone hypoacetylation act synergistically to achieve a highly stable inactive state.
Materials and Methods
Mice and Preparation of Mouse Embryonic Fibroblasts
The Xist2lox(Csankovszki et al. 1999), the XistΔ (Marahrens et al. 1997), the GFP mice (Hadjantonakis et al. 1998), and the HprtΔ mice (Hooper et al. 1987) have been described elsewhere. To obtain mice carrying the GFP transgene and the Xist2lox allele in cis, germline recombinants were generated from double heterozygous females. Recombination frequency was 40% (n = 115). Similarly, we obtained mice with the HprtΔ and XistΔ alleles in cis from mice heterozygous for both mutations in trans (27% recombination frequency, n = 81). Finally, XistΔ;HprtΔ/Xist+;HprtΔ females were mated to Xist2lox;Hprt+;GFP/Y males to generate Xist conditional mutant fibroblasts and Xist+;Hprt+;GFP/Y males to generate controls. The Dnmt2lox(Jackson-Grusby et al. 2001) and DnmtS(Lei et al. 1996) mutations were bred into the colony to create Xist, Dnmt1 double conditional knockout fibroblasts.
Primary mouse embryonic fibroblasts were derived from dissociation and trypsinization of embryonic day 14 embryos, cultured, and when necessary immortalized with SV-40 T-antigen (Jat et al. 1986). For Cre-mediated recombination in fibroblasts, cells were infected with an adenovirus vector carrying the gene for Cre recombinase (Anton and Graham 1995). Infection was carried out in monolayer culture in DME with 2% fetal calf serum for 2 h. The lowest possible multiplicity of infection that yielded 100% recombination without cytotoxic effects was experimentally determined. Uninfected cells were treated identically, without the addition of virus. After infection, cells were grown in DME with 15% fetal calf serum with antibiotics. When appropriate, 5-azadC (Sigma-Aldrich) was added to the cultures to a final concentration of 0.3 μM, and TSA (Sigma-Aldrich) to final concentration of 500 nM.
To analyze the efficiency of Cre-mediated Xist deletion, genomic DNA of infected cells was digested with XbaI, blotted, and hybridized with probe 7, a 1.1-kb EcoRI-XbaI fragment at the beginning of exon 7. To analyze recombination at the Dnmt1 locus, genomic DNA was digested with SpeI and hybridized with the HV probe (Jackson-Grusby et al. 2001). To analyze demethylation of genomic DNA, an HpaII digest was performed, and the blot was hybridized with a probe covering the gag coding region of intracisternal A particle (IAP) element (nucleotides 1570–1899, sequence data available from GenBank/EMBL/DDBJ under accession no. M17551) (Walsh et al. 1998).
Fibroblast cultures were trypsinized to obtain single cell suspension and resuspended in complete medium. Propidium iodide was added to 1 μg/ml. Viable cells were gated using scatter properties and exclusion of propidium iodide. 100,000–500,000 cells were analyzed for each bulk sample and 10,000 cells for poorly growing hypoxanthine/aminopterin/thymidine (HAT)–resistant clones. To isolate GFP-positive clones, single GFP-positive cells were sorted into wells of a 96-well plate containing DME with 15% fetal calf serum. After 2 wk, 20–30% of the wells contained fibroblast clones, of which ∼30% were GFP-positive or contained a high percentage of GFP-positive cells.
HAT Selection and Calculation of Reactivation Frequencies
For selection of clones carrying a reactivated Hprt gene, the appropriate number of cells were plated and selected in 1× ESQ HAT (Stratagene) containing media for 14 d. After selection, HAT-resistant clones were picked into regular media. For counting the number of HAT-resistant clones, plates were fixed in methanol/acetic acid (3:1) and stained with Giemsa. For Luria-Delbrück fluctuation analysis (Luria and Delbrück 1943), small independent fibroblast cultures were expanded to the appropriate size, plated at a density equivalent of a 1:9 to 1:6 split in HAT containing medium, and selected, fixed, and stained as above. Reactivation rates were calculated according to the P0 method of Luria and Delbrück 1943 (rate = −ln[proportion of negative cultures]/average culture size).
Analysis of Replication Timing
Cells were grown in the presence of 30 μM BrdU for the last 5 h before fixation. Colcemid (Sigma-Aldrich) was added for the last hour. Cells were fixed in methanol/acetic acid (3:1) and dropped onto slides. Slides were denatured in 70% formamide/2× SSC at 70–74°C for 2 min. BrdU signal was detected using a monoclonal anti-BrdU antibody (Becton Dickinson) followed by fluorescein-conjugated anti–mouse antibody (Vector Laboratories) in blocking buffer (1× PBS, 5% goat serum, 0.2% Tween, 0.2% fish skin gelatin). Slides were washed in 1× PBS/0.2% Tween, dehydrated, and used for DNA FISH without further denaturation of the chromosomes. The Xi was identified with a directly labeled GFP/Pgk-Puro probe. The inserts of EGFP-N1 plasmid (CLONTECH Laboratories, Inc.), and pPGKPuro were isolated, pooled, and labeled with Cy3-dCTP (Amersham Pharmacia Biotech) using random priming. Using only the GFP insert as a probe yielded identical results, but the signals were weaker. Only results obtained with the GFP/Pgk-Puro probe are shown. Hybridization of the probe and washing were performed as described (Panning and Jaenisch 1996).
Generation of Xist Mutant Mouse Embryonic Fibroblasts
To study the stability of silencing on Xi, we generated fibroblasts with two Xi-linked markers, where reactivation was designed to be detectable even at low frequencies. One marker was an X-linked GFP transgene that is subject to X inactivation (Hadjantonakis et al. 1998). When the GFP transgene was located on Xi, cells were GFP negative and reactivation could be monitored using FACS® analysis. The insertion site of the transgene was determined by DNA FISH, and GFP was mapped to a position near the centromere (Fig. 1 A, and see Fig. 5 A). The second marker was the endogenous X-linked Hprt gene, the activity of which is required in order to survive in HAT containing medium. When cells carrying a wild-type Hprt allele on Xi and a mutant allele, HprtΔ (Hooper et al. 1987), on the active X (Xa) are subjected to HAT selection, even a few reactivants in a large population can be isolated. To generate a homogeneous population of cells with defined Xa and Xi chromosomes, a null mutation in the Xist gene, XistΔ (Marahrens et al. 1997), was introduced onto the chromosome carrying HprtΔ. Since the XistΔ allele cannot be chosen for X inactivation (Marahrens et al. 1998), cells with genotype Hprt+;GFP/XistΔ;HprtΔ carry the GFP transgene and the Hprt+ allele on Xi.
To study the effect of deletion of Xist from Xi, a conditional allele of the gene Xist2lox (Csankovszki et al. 1999) was introduced onto the chromosome. Cells with genotype Xist2lox;Hprt+;GFP/XistΔ;HprtΔ will be referred to as conditional mutants. Control cells with genotype Xist+;Hprt+;GFP/XistΔ;HprtΔ lack the Xist2lox allele, and therefore cannot delete the Xist gene (Fig. 1 B). To induce Cre-mediated deletion of Xist2lox, we infected cells with an adenovirus carrying the gene encoding Cre recombinase (Anton and Graham 1995). An Xist2lox to Xist1lox recombination was observed in 100% of the cells, as assayed by Southern blotting (Fig. 1 C). Conditional mutants and controls were treated identically, and infections and all further analyses were done in triplicate. Cre-mediated deletion of Xist took place over a period of 2–3 d, and Xist RNA levels were undetectable by day 4 (Csankovszki et al. 1999; data not shown). In a previous study, we showed that deletion of Xist in mouse embryonic fibroblasts does not interfere with late replication timing and underacetylation of histone H4 residues, but it disrupts preferential localization of histone macroH2A1 to Xi (Csankovszki et al. 1999).
Deletion of Xist Leads to Increased Reactivation of GFP and Hprt
GFP expression was analyzed using FACS® in Xist mutant and control cells that were infected with adenovirus-Cre or left untreated. GFP fluorescence was compared with autofluorescence, and cells showing greater GFP fluorescence than autofluorescence were counted as positive. We found that the number of cells expressing GFP was dependent on cell density and both the number of cells expressing GFP and the intensity of fluorescence decreased upon long term culture (data not shown). Therefore, care was taken to ensure that an equal number of cells were plated for each sample and cells from the same early passage were used for each experiment. Results of a typical experiment are shown in Fig. 2. Fibroblasts not containing the GFP transgene (genotype +/Y) were negative, whereas over 99.9% of cells with GFP on Xa (GFP/Y) were positive. The majority of cells with GFP on Xi were also GFP negative with a small number of positives, ∼10–20 in 100,000, representing the spontaneous reactivation frequency (Fig. 2 A). In primary Xist conditional mutant fibroblasts after Cre-mediated deletion of Xist, the number of GFP-positive cells increased about twofold (Fig. 2 B). This increase cannot be attributed to the effect of adenovirus infection, as the number of GFP-positive cells did not increase in control cells after viral infection. Although the effect is small, we consider it significant as we consistently detected a twofold difference in GFP expressing cells between mutant and control cells in five independent repetitions of the assay.
We considered the possibility that allowing the cells to go through many rounds of cell division in the absence of Xist will lead to an increased number of cells reactivating GFP. To test this hypothesis, we derived permanent cell lines by SV-40 T-antigen transformation and cultured the cells for over 2 mo. GFP expression was analyzed at various time points (Fig. 2 C). 7 d after adenoviral infection, the transformed cells behaved similarly to primary cells: the conditional mutants exhibited a two- to threefold increase in the number of GFP-positive cells after Cre-mediated deletion of Xist, whereas there was no difference between infected and uninfected control cells. However, by day 14 after infection, the difference between the infected and uninfected mutant cells disappeared, and the proportion of GFP-positive cells remained unchanged for >2 mo. Reactivated GFP alleles are likely subject to resilencing, consistent with our observations that GFP expression declines over time and with earlier studies that showed that this transgene is subject to nonspecific silencing, even when carried on Xa (Eggan et al. 2000). In addition, it is possible that reactivation of X-inactivated genes confers selective disadvantage on the cells leading to a decrease in the number of GFP-positive cells over time (see below).
Next, we analyzed reactivation of an endogenous X-inactivated gene, Hprt, by subjecting cells to selection in HAT medium. Since HAT-resistant colonies from rare reactivants can only be obtained in permanent cell lines, these experiments were performed in SV-40 T-antigen–immortalized cells. Two million cells were plated and selected in HAT medium for 2 wk, after which plates were fixed and stained to count the number of colonies (Fig. 3 A). Very few (<1/plate) colonies were seen on control plates and on plates containing conditional mutant fibroblasts before Cre-mediated Xist, indicating that the spontaneous reactivation frequency of Hprt is very low. However, after deletion of Xist, a small but significant number of cells reactivated Hprt, and Xist mutant cultures yielded ∼30–70 HAT-resistant colonies per plate. The proportion of HAT-resistant cell in the population increased for the first 4 wk in culture indicating ongoing reactivation of Hprt. Furthermore, HAT-resistant cells were detected even after 3 mo in culture (Fig. 3 B). Northern analysis of total RNA indicated that different clones transcribed different amounts of Hprt RNA (data not shown). We conclude that deletion of Xist leads to an increased, albeit low, frequency of reactivation of an endogenous X-inactivated gene, Hprt, indicating that Xist RNA contributes to stabilizing the inactive state in the maintenance phase of X inactivation.
Patchy Reactivation of X-inactivated Genes in Xist Mutant Fibroblasts
As the nature of Xist RNA–mediated silencing has not been studied in detail in somatic cells, we next examined whether Xist RNA coordinately silences genes on Xi or whether genes are regulated independently of one another. First, we isolated HAT-resistant clones with a reactivated Hprt allele and asked whether these cells are also GFP-positive (Fig. 4). We analyzed two types of clones, fast-growing ones that grew almost as well as the unselected population (n = 6), and slow-growing ones that divided barely enough to yield sufficient cells for FACS® analysis (n = 7). In Xist mutant and Xist wild-type bulk populations before HAT selection, the number of GFP-positive cells was ∼1 in 10,000. Among fast-growing clones, the variation was large, but on average the clones contained 10–20 times more GFP-positive cells than the unselected populations. In slow-growing clones, the number of GFP-positive cells was on average another 10-fold higher (Fig. 4). Yet, even in the clones with the highest proportion of GFP-positive cells, over 98% of cells remained GFP negative. Therefore, most cells that reactivated Hprt generally did not also reactivate GFP. However, a chromosome that reactivated Hprt was more prone to reactivate GFP than a chromosome with an inactive Hprt gene.
It is interesting to note that HAT-resistant clones with a higher proportion of GFP-positive cells grew slower than those with fewer GFP-positive cells. This result is consistent with the conclusion that reactivation of X-inactivated genes confers selective disadvantage on the cells. In clones with a higher proportion of GFP-positive cells, the more extensive reactivation is more detrimental to cell growth.
Finally, we isolated GFP-positive clones by sorting and expanding individual GFP-positive cells, and tested whether these clones also reactivated Hprt. Similarly to the HAT-resistant clones, GFP-positive clones did not grow well, and most died under HAT selection without yielding a single colony. However, occasionally (2 of the 42 clones analyzed), the clone grew well in HAT-containing medium, indicating that most, if not all, cells of the clone were also Hprt positive. We conclude that most clones that reactivated one X-linked gene do not also reactivate another. Yet, there is a certain level of cooperativity in reactivation, as a chromosome that reactivated one gene on Xi, is more likely to reactivate another one than a chromosome that has not reactivated any gene.
X Chromosomes with Reactivated Genes Remain Late Replicating
An Xi chromosome after deletion of Xist remains late replicating when analyzed in bulk population with presumably very few of the cells containing reactivated genes (Csankovszki et al. 1999). We wished to see whether in the reactivated clones, Xi, or a cytologically visible portion of it, became early replicating. We analyzed two slow-growing HAT-resistant clones with a high proportion of GFP-positive cells and one GFP-positive clone that was also HAT resistant. As the rest of the clones grew too poorly to obtain sufficient numbers of cells for the assay, we pooled small HAT-resistant colonies and GFP-positive clones, and the assay was also performed on the pools. BrdU incorporation into late-replicating regions was detected using an anti-BrdU antibody and Xi was identified by DNA FISH using a probe that detects the GFP transgene. In all clones and pools analyzed, the Xi marked by the GFP transgene was late replicating (Fig. 5B and Fig. C). These results indicate that even after reactivating one or more genes on Xi, the chromosome as a whole remained inactive. We conclude that reactivation of Xi-linked genes after loss of Xist RNA occurs at one or a few loci and does not result in a detectable change in late replication of the chromosome.
Synergism of Xist RNA, DNA Methylation, and Histone Hypoacetylation in X Chromosome Silencing
Next, we examined the relationship between Xist RNA-mediated silencing and inactivation by other mechanisms. DNA methylation and hypoacetylation of core histones are believed to contribute to inactivation of X-linked genes (Cedar 1988; Keohane et al. 1998). A low frequency of reactivation of X-linked genes has been observed after demethylating cells using 5-azadC (Mohandas et al. 1981; Graves 1982). Transcriptional activation of silenced genes has also been seen after treating cells with TSA, a potent inhibitor of histone deacetylases (Yoshida et al. 1995). We wanted to see whether the Xist mutant cells with their already compromised ability to silence Xi are more sensitive to demethylation and/or inhibition of histone deacetylation than wild-type cells, leading to a further increase in the number of cells reactivating GFP and Hprt.
Adenovirus-Cre–infected and –uninfected Xist conditional mutant cells were treated with 5-azadC and/or TSA, and the number of cells that reactivated GFP was analyzed using FACS® (Fig. 6 A). Due to the toxicity of the drugs, the experiments were performed in SV-40 T-antigen–transformed cells. The cells were infected with adenovirus-Cre, allowed to recover, and then treated twice with 5-azadC on days 7 and 9 after infection. After allowing the cells to go through several rounds of cell division to achieve demethylation of DNA, half of the cultures were treated with TSA on day 12 after infection. FACS® analysis was performed on day 13. By day 13 after infection, the Xist deletion–induced increase in the number of GFP reactivants disappeared, and we could no longer observe a difference between Xist wild-type and Xist-deficient cells without drug treatment (Fig. 2 C). Inhibition of histone deacetylases by itself had no effect on the number of GFP-positive cells, whether or not Xist was deleted. 5-azadC–induced demethylation increased the number of GFP-positive cells by ∼20-fold in cells that did not delete Xist. However, the combined effect of Xist deletion and 5-azadC treatment was a 30–40-fold increase in GFP reactivants. 5-azadC treatment followed by TSA further increased the number of GFP-positive cells by another twofold in both Xist mutant and control cells. These results are summarized in Table. The ≤60-fold increase in the number of cells reactivating GFP indicates that the effects of Xist RNA deletion, 5-azadC, and TSA treatments are synergistic, rather than simply additive.
5-azadC treatment leads to limited genomic demethylation (Fig. 7 A). More extensive demethylation can be achieved by deleting Dnmt1. To study how X inactivation is maintained in the absence of Xist RNA and DNA methylation, we bred a Dnmt1 conditional allele (Jackson-Grusby et al. 2001) into the Xist mutant colony and generated double conditional mutant fibroblasts. Fibroblast genotypes were Xist2lox;GFP/XistΔ,Dnmt12lox/S, for Xist conditional mutants, and Xist+;GFP/XistΔ,Dnmt12lox/S, for control. The Dnmt1S allele is a constitutive null mutation of the gene (Lei et al. 1996). Upon adenovirus-Cre infection of these cells, both Xist and Dnmt1 were deleted in Xist mutant cells, whereas only Dnmt1 was deleted in the controls (Fig. 7 B). Deletion of Dnmt1 led to a more pronounced demethylation of bulk genomic DNA than 5-azadC treatment (Fig. 7). Primary Dnmt1 mutant fibroblasts arrested within 1 wk of adenovirus-Cre infection, whereas SV-40 T-antigen–transformed cells continued dividing, although at a much slower rate than wild-type cells (Jackson-Grusby et al. 2001). We analyzed both primary and transformed cells 7 d after infection. A much higher proportion of cells reactivated GFP in the Dnmt1 mutants than in 5-azadC–treated cells (Fig. 6 B), most likely as a result of the Dnmt1 mutants being much more demethylated. Transformed cells consistently yielded more GFP, reactivants possibly because of their increased ability to proliferate and further demethylate or as a result of decreased stability of silencing in transformed cells. Xist/Dnmt1 double mutants reactivated GFP in about twice as many cells as Dnmt1 single mutants, indicating again that Xist and DNA methylation cooperate to silence GFP on Xi. GFP was reactivated in ≥30% of Dnmt1/Xist double mutant cells, representing an almost 3,000-fold increase over controls (Table). Interestingly, the Dnmt1 mutation, or even limited demethylation using 5-azadC, has a much more significant effect on the number of GFP reactivants than the Xist mutation, arguing that at least for the X-linked GFP transgene, DNA methylation is a more important contributor to silencing than Xist.
To study the combined effect of demethylation and Xist deletion on an endogenous X-inactivated gene, we analyzed Hprt reactivation in adenovirus-Cre–infected or –uninfected Xist conditional mutant cells, with or without 5-azadC treatment (Fig. 6 C). In adenovirus-Cre–infected (Xist deleted) cultures without drug treatment, we observed an ∼100-fold enrichment for HAT-resistant cells over uninfected (Xist wild type) cells. 5-azadC treatment of Xist wild-type cells resulted in a less significant 10-fold increase in the number colonies per plate. However, 5-azadC treatment of Xist mutant cells resulted in a 50-fold increase in HAT-resistant cells over untreated Xist mutant cells and an almost 5,000-fold increase over untreated Xist wild-type cells (Table). The combined effect of Xist deletion and demethylation is more significant than either treatment alone, implying a synergistic interaction of Xist RNA and DNA methylation in keeping Hprt silent. It is interesting to note that although the absolute numbers of GFP- and Hprt-positive cells are different, 5-azadC treatment led to comparable enrichment in reactivants for both genes (19- and 12-fold, respectively). However, Xist RNA seems to play a more major role in Hprt silencing than in GFP silencing (100-fold enrichment compared with two- to threefold enrichment). The GFP transgene may not be subject to Xist RNA–mediated silencing the same way endogenous X-linked genes are regulated.
Rate of Hprt Reactivation in Xist-deficient Fibroblasts
To test whether the observed HAT-resistant colonies are the result of independent Hprt reactivation events or proliferation of a few reactivants, we calculated Hprt reactivation rates using the Luria-Delbrück fluctuation analysis (Luria and Delbrück 1943). A large number of cultures of adenovirus-Cre–infected and –uninfected cells were expanded from a few cells (generally <100). During expansion, half of the cultures were treated with 5-azadC. After the desired culture size was reached, cells were selected using HAT, and the number of cultures that yielded HAT-resistant colonies and the reactivation rates were determined (Table). The positive cultures ranged from those containing one clone to those containing confluent plates, indicating that the reactivation event took place at different times during cultivation. The spontaneous reactivation rate of Hprt was as low as previously reported mutation rates in wild-type cells (10−9) (Chen et al. 1998), demonstrating the remarkable stability of X chromosome silencing. The reactivation rate increased by ∼160-fold after deletion of Xist and 60-fold after 5-azadC treatment, indicating that both Xist RNA and DNA methylation contribute significantly to silencing. However, combining Xist deletion with 5-azadC treatment resulted in an almost 10,000-fold increase, confirming synergism of DNA methylation and Xist expression in the maintenance of the inactive state.
We generated fibroblasts in which reactivation of two genes on the X chromosome, a GFP transgene and the endogenous Hprt gene, can be detected at a low frequency. We studied the effect of loss of Xist RNA, demethylation of genomic DNA and inhibition of histone deacetylation, on the maintenance of X inactivation. We observed that deletion of Xist leads to reactivation of GFP and Hprt in a very small proportion of cells and conclude that Xist, though not essential for the maintenance of X inactivation, contributes to the stability of the inactive state. We further showed that Xist RNA, histone deacetylation, and DNA methylation act synergistically to achieve the extraordinary stability of X chromosome silencing, with reactivation rates comparable to mutation rates.
Synergism of X Inactivation Mechanisms
It has been shown that during the early stages of cellular differentiation, an Xist RNA–mediated silencing mechanism initiates X inactivation (Penny et al. 1996; Marahrens et al. 1997; Wutz and Jaenisch 2000), and that Xist becomes dispensable for the maintenance of X inactivation after subsequent differentiation (Brown and Willard 1994; Rack et al. 1994, Csankovszki et al. 1999). However, we now present direct evidence that an Xist RNA–mediated maintenance mechanism contributes to silencing in somatic cells. Deletion of Xist reduces the histone macroH2A1 content of Xi chromatin (Csankovszki et al. 1999), and it is possible that this change in histone composition leads to compromised efficiency of silencing. However, to directly assess the role of histone macroH2A1 in X chromosome inactivation, analysis of a targeted mutation of the gene will be necessary.
DNA methylation is another significant contributor to silencing. Demethylation by 5-azadC has been used before to reactivate genes on Xi (Mohandas et al. 1981; Graves 1982). In this study, we also introduced a Dnmt1 mutation that proved to be ∼100 times as effective as 5-azadC treatment in achieving reactivation of GFP. Demethylation combined with Xist deletion increased reactivation rates to a greater extent than either did alone, indicating synergism of silencing mechanisms in keeping Xi silent. In the case of the GFP transgene, we accomplished ≥30% reactivation in Xist/Dnmt1 double mutant fibroblasts. However, at least in the case of Hprt, the majority of the cells maintained silencing even after deletion of Xist and demethylation, indicating the presence of additional stabilizing mechanisms, such as late replication.
Partial compensation for reduced methylation on Xi by other silencing mechanisms occurs in ICF patients. Xi in these patients lacks methylation on CpG islands (Hansen et al. 2000) and, therefore, presumably histone deacetylation is also compromised. However, Xist RNA localizes normally to Xi and, together with late replication, is able to maintain X inactivation, although with reduced efficiency (Hansen et al. 2000).
Inhibition of histone deacetylation by TSA led to a small increase in the number of GFP reactivants. One possible explanation for the modest effect of histone deacetylase inhibitors is the slow rate of histone acetate turnover on the Xi of differentiated cells leading to limited enrichment in acetylated histones after TSA treatment (Keohane et al. 1998). Indeed, treatment of cells with another histone deacetylase inhibitor, sodium butyrate, did not increase antiacetylated histone staining on Xi (Jeppesen and Turner 1993). Furthermore, TSA only inhibits GFP silencing in demethylated cells. A similar dependence of reactivation of genes by TSA on demethylation has been observed by others studying genes silenced in cancer (Cameron et al. 1999), implying that in these cases DNA methylation is the primary mechanism that recruits histone deacetylases to the silenced loci, possibly via binding of methyl-DNA binding proteins (Jones et al. 1998; Nan et al. 1998). In other cases, histone deacetylase inhibitors alone were sufficient to achieve reactivation, such as reexpression of the FMR1 gene in cells derived from fragile X syndrome patients, whereas synergism of histone deacetylation and DNA methylation was still observed (Chiurazzi et al. 1999).
The synergism of multiple silencing mechanisms to assure a highly stable repressed state possibly reflects the importance of dosage compensation for the proper functioning of the organism. It has been demonstrated that gene dosage imbalance in the embryo (Takagi and Abe 1990), or in the extraembryonic tissues (Marahrens et al. 1997), causes lethality. However, partial reactivation of the chromosome appears to be tolerated in vitro, and it is possible to isolate and culture cells with reactivated X-linked genes. Yet, our fibroblast clones with reactivated Xi-linked genes grew more poorly than fibroblasts of the same genotype that did not reactivate any gene. These results argue that gene dosage imbalance is detrimental to cell growth even in vitro and that clones that reactivated the entire chromosome may not be viable. Therefore, our calculations of reactivation frequencies might be an underestimation, as cells with reactivated chromosomes may die before they can be detected.
Xist RNA and DNA Methylation Contribute Differently to Silencing of Two X-linked Genes
The two genes analyzed, GFP and Hprt, are both subject to X inactivation, but the reactivation rates are different. In the presence of Xist RNA and wild-type levels of methylation and histone H4 acetylation, Hprt is almost never reactivated, whereas GFP reactivation can be readily observed. The difference can be at least partially attributed to the difference in assays. Although reactivation of GFP can be observed almost instantly on FACS®, detection of Hprt reactivants by HAT selection requires that the cells survive reactivation and maintain their proliferative capacity. The smallest detectable HAT-resistant colony contained ∼30 cells, the result of about five cell divisions.
The transgenic nature of GFP might also influence the way the gene responds to silencing mechanisms. Xist RNA may not be able to exert the same level of control over a transgene as over endogenous genes, therefore deletion of Xist has a smaller effect on GFP reactivation than on Hprt reactivation. On the other hand, DNA methylation contributes significantly to the silencing of both genes. Randomly integrated transgenes are frequently methylated (Hertz et al. 1999), which may contribute to their variable expression. GFP is integrated near the centromere and therefore might also be subject to silencing by centric heterochromatin. Nonspecific silencing of GFP by mechanisms unrelated to X inactivation (Eggan et al. 2000) may explain the rapid disappearance of GFP reactivants from the cultures. The observed influence of different mechanisms on Hprt may more faithfully represent silencing of endogenous X-inactivated genes.
Mechanism of X Chromosome Silencing
In recent years, significant progress has been made in deciphering how DNA and histone modifications regulate transcription. Methylation of DNA is thought to change accessibility of chromatin via binding of methylated DNA binding proteins that in turn can recruit histone deacetylases (Jones et al. 1998; Nan et al. 1998). Acetylated NH2-terminal lysines of histones, aside from affecting compactness of chromatin packaging, can bind the bromodomain module present in a wide range of chromatin remodeling proteins (Dhalluin et al. 1999; Jacobson et al. 2000).
The mechanism of Xist RNA–mediated silencing is not as well understood. Xist RNA is involved in preferential localization of histone macroH2A1 to Xi (Csankovszki et al. 1999). However, we do not know whether histone macroH2A1 and Xist RNA interact directly and to what extent histone macroH2A1 participates in silencing. It has been shown that Xist RNA can silence in the absence of DNA methylation (Panning and Jaenisch 1996), or even before cellular differentiation (Wutz and Jaenisch 2000). Xist RNA can also accomplish transcriptional silencing without the chromosome becoming late replicating or hypoacetylated (Wutz and Jaenisch 2000). This study provides evidence that the Xist RNA–mediated silencing mechanism acts synergistically with other silencing factors. Xist RNA, similarly to DNA methylation, appears to act in a localized manner, not as a master switch regulating the entire chromosome. Our observations on the effects of deletion of Xist and earlier studies on 5-azadC reactivated clones (Mohandas et al. 1981; Graves 1982) indicate that reactivation of genes on Xi is neither coordinate nor independent, as reactivation of one gene correlates with reactivation of other linked genes only to a limited extent. Xist mutant clones with reactivated genes, in which the lack of Xist RNA–mediated silencing has phenotypic consequences, provide a useful reagent for further dissecting out how Xist RNA might accomplish silencing.
We thank Glen Paradis for help with FACS®; Nicki Watson for help with microscopy; David Humpherys for the preparation of the IAP probe; and Anton Wutz, Ted Rasmussen, Sandra Luikenhuis, and David Akey for discussions and critical reading of the manuscript. This work was conducted using the W.M. Keck Foundation biological imaging facility at the Whitehead Institute.
The work was supported by a grant to R. Jaenisch from the National Institutes of Health/National Cancer Institute (R35-CA44339).
Abbreviations used in this paper: GFP, green fluorescent protein; HAT, hypoxanthine/aminopterin/thymidine; Hprt, hypoxanthine phosphoribosyl transferase; IAP, intracisternal A particle; ICF, immunodeficiency centromeric instability facial anomalies; TSA, trichostatin A; Xa, active X; Xi, inactive X.