Gene name - Histone H3.3A
Cytological map position - 25C3
Function - chromatin protein
Keywords - replacement histone, nucleosome assembly associated with transcriptional activation
Symbol - His3.3A
FlyBase ID: FBgn0014857
Genetic map position - 2L
Classification - Histone H3
Cellular location - nuclear
|Recent literature||Paranjape, N. P. and Calvi, B. R. (2016). The histone variant H3.3 is enriched at Drosophila amplicon origins but does not mark them for activation. G3 (Bethesda) [Epub ahead of print]. PubMed ID: 27172191
Eukaryotic DNA replication begins from multiple origins. The origin recognition complex (ORC) binds origin DNA and scaffolds assembly of a pre-Replicative Complex (pre-RC), which is subsequently activated to initiate DNA replication. In multicellular eukaryotes, origins do not share a strict DNA consensus sequence and their activity changes in concert with chromatin status during development, but mechanisms are ill-defined. Previous genome-wide analyses in Drosophila and other organisms have revealed a correlation between ORC binding sites and the histone variant H3.3. This correlation suggests that H3.3 may designate origin sites, but this idea has remained untested. To address this question, this study examined the enrichment and function of H3.3 at the origins responsible for developmental gene amplification in the somatic follicle cells of the Drosophila ovary. H3.3 was found to be abundant at these amplicon origins. H3.3 levels remained high when replication initiation was blocked, indicating that H3.3 is abundant at the origins before activation of the pre-RC. H3.3 was also enriched at the origins during early oogenesis, raising the possibility that H3.3 bookmarks sites for later amplification. However, flies null mutant for both of the H3.3 genes in Drosophila did not have overt defects in developmental gene amplification or genomic replication, suggesting that H3.3 is not essential for the assembly or activation of the pre-RC at origins. Instead, the results imply that the correlation between H3.3 and ORC sites reflects other chromatin attributes that are important for origin function.
DNA in eukaryotic cells is packaged into nucleosomes, the structural unit of chromatin. Both DNA and bulk histones are extremely long-lived, because old DNA strands and histones are retained when chromatin duplicates. In contrast, the Drosophila HSP70 genes rapidly lose histone H3 and acquire variant H3.3 histones as these genes are induced. Histone replacement does not occur at artificial HSP70 promoter arrays, demonstrating that transcription is required for H3.3 deposition. The H3.3 histone is enriched in all active chromatin and throughout large transcription units, implying that deposition occurs during transcription elongation. Strikingly, the stability of chromatin-bound H3.3 differs between loci: H3.3 turns over at continually active rDNA genes, but becomes stable at induced HSP70 genes that have shut down. It is concluded that H3.3 deposition is coupled to transcription, and continues while a gene is active. Repeated histone replacement suggests a mechanism to both maintain the structure of chromatin and access to DNA at active genes (Schwartz, 2005).
Transcriptional regulation in eukaryotes requires the coordinated recruitment of RNA polymerase II along with a variety of activators, repressors, chromatin-remodeling factors, and other chromatin-associated proteins. Histone variants have also been implicated in transcriptional regulation. All eukaryotic genomes encode four conserved core histones that package bulk chromatin, but a fraction of chromatin is packaged by alternate histones. Three lines of evidence support the argument that an alternate H3 histone subtype in animals -- the variant H3.3 -- plays a role in transcriptionally active chromatin: (1) a pulse of epitope-tagged H3.3 protein localized to gene-rich chromatin in Drosophila cells (Ahmad 2002); (2) H3.3 became enriched at a transgene array after its induction (Janicki, 2004); (3) H3.3 is enriched for covalent histone modifications associated with active chromatin, while repressive modifications are enriched on the H3 histone (McKittrick, 2004). These observations suggest that H3.3 is a common component of active chromatin (Schwartz, 2005).
Studies of the H3.3 variant have also suggested that distinctive nucleosome assembly occurs in active chromatin. Recent biochemical and in vivo assays demonstrate that there are both DNA replication-coupled and replication-independent (RI) nucleosome assembly pathways in eukaryotic nuclei. DNA replication-coupled assembly serves to package newly synthesized DNA into nucleosomes, but the existence of RI assembly pathways implies that previously chromatinized templates are also loading new histones. One RI pathway exclusively deposits newly synthesized histone H4 and the H3.3 variant and operates specifically at active chromatin in interphase nuclei (Ahmad, 2002; Tagami, 2004). However, the relationship between transcriptional activity and H3.3 has not been defined. It is unknown if H3.3 deposits during or after transcription of a gene, or how frequently RI assembly occurs. Conceivably, occasional RI assembly would have little effect on the physical properties of chromatin and the stability of histone modifications. Alternatively, the structure of active chromatin might be disrupted if RI assembly occurs frequently (Schwartz, 2005).
This study demonstrates that H3.3 deposition is triggered by gene induction, and deposition occurs while genes are transcribed. H3.3 deposition is also associated with histone removal and degradation that depends on the activity of a locus. Repeated rounds of replacement may function to destabilize active chromatin. The progressive degradation of H3.3 histone subtypes is distinct from the conservative exchange of H2A/H2B subtypes, and explains constitutive synthesis of new H3.3 histone (Schwartz, 2005).
Cells use two pathways for the assembly of nucleosomes. The replication-coupled pathway suffices to package the bulk genome as DNA is replicated, using histones synthesized from the major canonical genes. The RI pathway acts on transcriptionally active loci and specifically uses the H3.3 histone variant (Ahmad, 2002; Janicki 2004; Tagami 2004). This study shows that RI assembly begins within minutes after gene induction and operates while genes are active. The binding of transcription factors to artificial promoter arrays is insufficient to trigger H3.3 deposition, implying that RI assembly is tied to a late step in gene induction. The findings that H3.3 becomes distributed throughout long transcribed genes suggest that RNA polymerase progression itself is involved in histone displacement and replacement. Finally, the stability of H3.3 in chromatin depends on transcriptional status: At continually active loci, H3.3 deposits and then leaves, but when genes become repressed, incorporated H3.3 becomes stable. This dependence is explained if transcription causes the displacement of chromatin-bound histones (Schwartz, 2005).
In vitro experiments show that RNA polymerases often pause when they run into a nucleosome. Transcription through a nucleosome requires the transient disruption of histone-DNA contacts so that the polymerase can progress. A key question is whether the loss of these contacts releases histones from DNA as the polymerase passes, or if the histones remain associated. The current view is that accessory factors assist polymerases by moving histone octamers along the template, or by returning any histones that are displaced. However, the rapid stimulation of H3.3 replacement by gene induction implies that, at least sometimes, displaced histones are not restored. The enrichment of H3.3 at all active chromatin in Drosophila indicates that the loss of displaced histones is a general feature of transcription from chromatin templates (Schwartz, 2005).
There are two processes that might link histone variant replacement to transcription. (1) The polymerase may displace histones, thus producing a naked template suitable for RI assembly machinery. Such a dependence on prior nucleosome disassembly would effectively restrict H3.3 replacement to active genes. (2) Factors that accompany elongating RNA polymerase may catalyze histone replacement. Support for this idea comes from the detection of transcriptional regulators in isolated H3.3 predeposition complexes (Tagami, 2004). Tagami suggested that these regulators might serve as protein interfaces to recruit H3.3 to sites of active transcription. Indeed, a protein interaction between the histone chaperone CAF large subunit and the DNA replication fork protein PCNA serves to enhance replication-coupled deposition of histone H3 (Shibahara, 1999). An analogous role might be performed by transcription factors that interact with the HIRA chaperone in H3.3 predeposition complexes. Additionally, the histone-binding proteins SPT5 and SPT6 are known to localize to transiently induced HSP70 genes, and are thought to manipulate nucleosomes for transcription (Andrulis, 2000). Such factors might drive histone replacement to clear DNA for polymerase passage. SPT5 and SPT6 are not known to localize to sites of RNA Pol I transcription, so there may also be analogous polymerase-specific factors that clear DNA. Since SPT5 and SPT6 leave HSP genes after transient induction, replacement would also cease and the genes would retain high levels of H3.3. Thus, H3.3 replacement leaves behind an extremely stable marker of past transcriptional activity (Schwartz, 2005).
The observation that chromatin-bound H3.3 has a short half-life (~24 h) is in stark contrast to the half-life of histones from bulk chromatin. Measurements of in vivo histone exchange have demonstrated recycling of H2A and H2B between sites within a nucleus, and at least one complex is capable of exchanging these histones between chromatin and histone chaperones. However, recycling of H3 and H4 was not detected, and in current experiments bulk H2B-GFP does not degrade. The fate of H3.3 when it is displaced from chromatin distinguishes H3.3 replacement from other kinds of chromatin exchange and remodeling, and suggests that replication-independent nucleosome assembly and disassembly is not an exchange reaction. This appears to be a general property of replacement H3 histones, because alfalfa replacement H3 also has a fast rate of turnover (Waterborg 1993). The rapid turnover of replacement H3 histones explains why all eukaryotes have constitutively expressed H3.3-type genes (Thatcher, 1994; Malik, 2003), because a continuous supply will be required to replenish active chromatin. Perhaps the purpose of specific histone degradation is to prevent exchange between chromatin sites. Chromatin-bound H3 and H4 are heavily modified, and it is suggested that H3/H4 subparticles are degraded to prevent moving modified histones to new sites. In contrast, the relative paucity of modifications on the H2A and H2B histones means that their exchange between sites has no detrimental effect (Schwartz, 2005).
Two other instances of histone degradation have been well-characterized. Chromatin-bound centromeric histones in budding yeast (CSE4) are subject to proteasome-mediated degradation that may limit this histone variant to centromeres (Collins 200). A separate system that degrades excess soluble histones has also been described (Gunjan, 2003). The current experiments do not distinguish whether H3.3 is degraded as it is displaced from chromatin or once it is soluble. Degradation of the histone may occur by a proteosome-catalyzed mechanism, or by a general response to damaged proteins. However, histone degradation in differentiated cells appears to discriminate between histone subtypes, because H2B-GFP is not similarly degraded. Since replication-independent histone deposition uses specialized chromatin assembly factors, the results raise the possibility that there are histone disassembly factors that specifically degrade H3.3. This could be tested with drugs that block known degradation pathways (Schwartz, 2005).
The H3 and H3.3 histones are extremely similar, differing by only four amino acid residues in Drosophila. Three of these specify whether the histone can be used for replication-coupled or RI nucleosome assembly, but these residues are not accessible in the complete nucleosome (Ahmad, 2002). This extreme similarity raises a paradox: What can be the function of replication-independent assembly, since new assembly results in a virtually identical nucleosome? In fact, the similarity between H3 and H3.3 distinguishes it from other histone variants like H2A.Z, which do introduce structural differences into the nucleosome. A possible resolution to this paradox comes from observations of the dynamics of RI assembly. Replication-coupled histone deposition only occurs once every cell cycle at a site, but RI deposition is a continual process at active genes. Thus, inactive chromatin retains the same histones for long periods of time, but active chromatin repeatedly shed its histones. Rapid turnover of histones at active genes has three implications for chromatin structure (Schwartz, 2005).
(1) The maintenance of any modification state in active chromatin will require ongoing activity of histone-modifying enzymes to modify newly arriving histones. Acetyl modifications do rapidly turn over in vivo, and can be removed enzymatically, but histone replacement will also contribute to turnover rates. Replacement may enhance the specificity of histone-modifying enzymes by continually removing modifications from active chromatin. Histone replacement also provides a mechanism to remove histone modifications that may not be metabolized. One example of this is the activation of heterochromatic gene arrays (Ahmad, 2002; Janicki 2004), where chromatin is marked by methylation at Lys 9 of the H3 tail (H3K9me). Activation of these gene arrays results in the coincident disappearance of H3K9me and deposition of H3.3, as if removal of the methylation mark occurs by histone replacement. In contrast, some histone modifications that are set during gene expression remain present after transcription and histone replacement ceases. Indeed, the retention of H3.3 at previously active chromatin may require that the variant maintain its extreme similarity with H3 so that they both can be repressed by the same modification systems (Schwartz, 2005).
(2) Continual histone replacement means that active regions have little time to 'mature' their chromatin between rounds of histone deposition. Nascent chromatin produced by replication-coupled assembly matures into a nuclease-resistant form within 1 h, and this delay is thought to reflect the rates for removing predeposition modifications, establishing new modifications, and condensing chromatin. If the rates for modification and condensation after RI assembly are similar to replicated chromatin, rapid histone turnover will continually reset chromatin to an 'immature' uncondensed state (Schwartz, 2005).
(3) High DNA accessibility is a characteristic feature of active chromatin, and this feature may simply result from ongoing histone replacement. This idea is supported by recent experiments in budding yeast demonstrating that the inducible accessibility of the PHO5 promoter is due to loss of nucleosomes. Earlier studies observed a slight decrease in the density of histone H4 at activated HSP70 genes, and concluded that transcription occurs without displacing histones from chromatin. However, a small decrease could result if displaced histones are rapidly replaced with new ones. Indeed, in budding yeast the density of histones appears to drop at very high transcription rates. Such transient structural instability of active chromatin would allow efficient polymerase elongation (Schwartz, 2005).
Most nucleosomes that package eukaryotic DNA are assembled during DNA replication, but chromatin structure is routinely disrupted in active regions of the genome. Replication-independent nucleosome replacement using the H3.3 histone variant efficiently repackages these regions, but how histones are recruited to these sites is unknown. This study used an inducible system that produces nucleosome-depleted chromatin at the Hsp70 genes in Drosophila to define steps in the mechanism of nucleosome replacement. Xnp chromatin remodeler and the Hira histone chaperone were found to independently bind nucleosome-depleted chromatin. Surprisingly, these two factors are only displaced when new nucleosomes are assembled. H3.3 deposition assays reveal that Xnp and Hira are required for efficient nucleosome replacement, and double-mutants are lethal. It is proposed that Xnp and Hira recognize exposed DNA and serve as a binding platform for the efficient recruitment of H3.3 predeposition complexes to chromatin gaps. These results uncover the mechanisms by which eukaryotic cells actively prevent the exposure of DNA in the nucleus (Schneiderman, 2012).
DNA in the eukaryotic nucleus is associated with histone proteins to form nucleosomes, the fundamental units of chromatin. Most nucleosomes are assembled during DNA replication, but chromatin structure is routinely disrupted in active regions of the genome. These regions are repackaged by replication-independent (RI) nucleosome replacement using the H3.3 histone variant. This process results in the enrichment of the H3.3 histone variant at all sites where nucleosomes are unstable or disrupted (Schneiderman, 2012 and references therein).
How H3.3 is delivered to dynamic chromatin sites is unknown. However, biochemical isolation of predeposition complexes has identified shared and distinctive assembly factors that associate with the H3 and H3.3 histones and mediate the replication-coupled or RI assembly of nucleosomes, respectively. These factors include histone chaperones and chromatin remodelers that are important for new nucleosome assembly, and might potentially target histones to active chromatin regions. However, mutants in some of these factors have surprisingly limited phenotypes. The Hira chaperone promotes H3.3 deposition at genes but is only essential for H3.3 deposition on sperm chromatin during fertilization. In Drosophila the ATRX/XNP remodeler homolog Xnp colocalizes with H3.3 in somatic cells, but is not essential (Schneiderman, 2009). In mammals, ATRX/XNP promotes H3.3 deposition only at telomeres and some heterochromatic sequences. These results have raised the possibilities that H3.3 assembly factors are redundant or that additional factors involved in the deposition of this histone variant exist. Loss of H3.3 itself can be compensated in somatic cells by the major H3 histone, suggesting that assembly of any nucleosome suffices (Schneiderman, 2012 and references therein).
This work used an inducible system that produces nucleosome-depleted chromatin at the Hsp70 genes in Drosophila to study the mechanism of nucleosome replacement. Evidence is provided that H3.3 predeposition factors mediate two separable steps in RI nucleosome assembly. The Xnp and Hira factors bind genomic sites when nucleosomes are disassembled, thereby marking sites for RI assembly. Strikingly, it was also demonstrated that Hira and Xnp are redundant for RI nucleosome assembly in somatic nuclei. The results further reveal that RI nucleosome replacement is essential for chromatin structure and viability, and uncover a cellular system that surveys chromatin for defects and promotes its repair (Schneiderman, 2012).
This study used the inducible Hsp70 genes as a controlled in vivo system to deplete nucleosomes from chromatin. Heat-shock activates transcription of Hsp70, displacing nucleosomes and increasing the sensitivity of the locus to digestion by micrococcal nuclease (MNase). After heat-shock, H3.3-containing nucleosomes repackage the locus. To generate persistently nucleosome-depleted chromatin, the Hsp70 genes in H3.3-deficient cells. ChIP experiments using an anti-H3 antibody show similar amounts of histone H3 at the Hsp70 genes in wild-type and H3.3-deficient salivary glands, and the genes show similar protection from MNase digestion. These data demonstrate that Hsp70 sequences are fully protected by nucleosomes before induction in wild-type and H3.3-deficient salivary glands. In both genotypes induced Hsp70 genes become hypersensitive to MNase as nucleosomes are lost. In wild-type cells after heat-shock nuclease protection is restored, but is not restored in H3.3-deficient glands. This finding demonstrates that nucleosomes are not replaced after Hsp70 induction in the absence of H3.3. This system allows the teasing apart of cause-and-effect in analyzing the effects of nucleosome assembly factors (Schneiderman, 2012).
Previous work has described that the Xnp chromatin remodeler colocalizes with H3.3 in chromatin (Schneiderman, 2009). Mammalian data has suggested that the Xnp homolog ATRX mediates H3.3 deposition at telomeres and at transcribed heterochromatic repeat sequences, although its nuclear distribution is much broader. The Hira histone chaperone has been implicated in global nucleosome replacement after the removal of protamines from the sperm nucleus during fertilization and near genes in mammalian cells. Purification of nuclear soluble H3.3-containing complexes showed that ATRX and Hira are in two separate complexes that mediate H3.3 deposition at distinct target sites. ASF1 is a general histone chaperone that complexes with new histone dimers in the cytoplasm and escorts them into the nucleu. This study used antibodies to Drosophila Xnp, Hira, and ASF1 to track their localization during Hsp70 induction and subsequent RI nucleosome assembly in polytene chromosomes of larval salivary glands (Schneiderman, 2012).
Heat-shock rapidly activates transcription of Hsp70, and elongating RNA polymerase II becomes strongly localized in puffs at the transcribing genes. After cessation of a heat-shock, the puffs regress and RNA polymerase II leaves the locus within 30 min. Neither Xnp, Hira, nor ASF1 were found to be enriched at the Hsp70 loci before induction. However, upon induction all three proteins are rapidly recruited to the Hsp70 loci. Xnp, Hira, and ASF1 remain associated with chromatin and the genes are transcribed, but then leave the Hsp70 genes after heat-shock. Their dynamic recruitment implicates these assembly factors in cotranscriptional nucleosome dynamics (Schneiderman, 2012).
The induction of Hsp70 was followed in H3.3-deficient salivary glands, where transcription produces nucleosome-depleted chromatin. Both Northern analysis and cytological observations of RNA polymerase II showed that Hsp70 was induced in wild-type and H3.3-deficient salivary glands, although H3.3-deficient glands produce ~50% less mRNA. Two effects on the recruitment of RI assembly factors were observed . First, Xnp, Hira, and ASF1 are all rapidly recruited to the induced Hsp70 genes at moderately reduced levels, indicating that the Hsp70 genes are less efficiently induced in this genotype. Second, both Xnp and Hira - but not ASF1 - accumulate and persist at the Hsp70 genes after heat-shock. The correspondence between persistent nucleosome depletion and the persistent binding of these factors is striking. This correspondence is a distinctive property of these two RI assembly factors, because the histone chaperone ASF1 is also cotranscriptionally recruited but dissociates both in wild-type and in H3.3-deficient cells. Finally, retention of Xnp and Hira is not a result of ongoing transcription, because RNA polymerase II rapidly leaves the Hsp70 loci after heat-shock and transcript production ceases. It is concluded that once Xnp and Hira bind nucleosome-depleted chromatin, they are only displaced when new nucleosomes assemble (Schneiderman, 2012).
How are Xnp and Hira recruited to nucleosome-depleted chromatin? These factors may be directly recruited by transcriptional machinery to active genes. Alternatively, Xnp and Hira may bind a structural feature common to chromatin gaps, or may simply bind exposed DNA. These factors might be complexed with DNA-binding factors or may bind DNA themselves. The homologous ATRX remodeler contains an ADD (ATRX-DNMT3-DNMT3L) domain that can bind DNA or histone tails. Indeed, ATRX is recruited to the genomes of DNA viruses as they enter the nucleus, suggesting that it may directly bind exposed DNA. A recent study has shown that the mammalian Hira chaperone may also directly bind exposed DNA at chromatin gaps. This study found that Xnp and Hira bind independently at induced Hsp70 genes in null mutants of the other factor, implying that there may be multiple ways that RI assembly factors recognize exposed DNA (Schneiderman, 2012).
Although both Xnp and Hira have been implicated in RI nucleosome assembly, mutants in these factors have surprisingly limited phenotypes. These results have raised the possibility that H3.3 assembly factors are redundant. To test if these factors promote nucleosome replacement at these sites, deposition of GFP-tagged truncated H3.3 histone into chromatin was assayed in wild-type and mutant genotypes. H3.3core-GFP can only be incorporated by RI nucleosome assembly, and the histone labels active genes.A pulse of H3.3core-GFP was produced in salivary glands and chromosome spreads were prepared 2 h later to assess the efficiency of RI nucleosome assembly. In wild-type cells, H3.3core-GFP strongly labels chromosome arms and active genes. In contrast, the H3.3core-GFP protein is efficiently produced in xnp-null mutant cells, but only a fraction of the protein deposits onto chromosomes; instead, most of the protein accumulates within the nucleolus. This protein does not coincide with DNA in the nucleolus, and may be predeposition or aggregated histones. Hira mutants have a similar reduction in H3.3 deposition: H3.3core-GFP protein is produced, but most protein accumulates in the nucleolus. These results demonstrate that the rate of RI nucleosome assembly is reduced in both xnp and Hira mutants, although some assembly can still occur. Indeed, longer expression of tagged histones in xnp or Hira mutants does achieve apparently normal levels (Schneiderman, 2012).
To test if Xnp and Hira have redundant roles in nucleosome replacement, Hira;xnp double-mutant animals were generated. Single-mutants are fully viable, but double-mutant larvae grow slower than wild-type siblings and die during larval development. Therefore H3.3core-GFP deposition was measured in these double-mutants. Strikingly, high levels of H3.3core-GFP were produced in Hira;xnp animals, but all of the protein accumulates in the nucleolus, with no detectable staining of chromosomes. It is concluded that both Hira and Xnp contribute to the efficiency of H3.3 RI nucleosome assembly, but this fails when both factors are eliminated (Schneiderman, 2012).
The results lead to the suggestion that Xnp and Hira identify nucleosome-depleted chromatin and promote new nucleosome assembly through a stepwise process (see Nucleosome-depleted chromatin gaps recruit assembly factors for the H3.3 histone variant). In the first step, Xnp and Hira bind exposed DNA at chromatin gaps, thereby marking sites where a nucleosome has been displaced. In the second step, delivery factors carrying new histones are recruited by binding to Xnp and Hira at chromatin gaps. In the final step, these factors assist in the transfer of histones from delivery chaperones to DNA, and Xnp and Hira are released when nucleosome assembly is complete (Schneiderman, 2012).
A previous study showned that the Xnp remodeler is found at all sites where H3.3 is enriched, including active genes (Schneiderman, 2009). The Hira chaperone also localizes at active genes. However, there are additional sites in the genome where the two assembly factors do not coincide. First, the major site for Xnp binding is at a nucleosome-depleted satellite block, where Hira is not found. Second, most Hira is localized to the repeated ribosomal DNA (rDNA) within the nucleolus, where Xnp is not found. This finding implies that the two factors are not redundant at all sites where H3.3 is deposited (Schneiderman, 2012).
The rDNA genes are repressed in late-stage salivary glands. Therefore, deposition of H3.3 was assayed in the somatic follicle cells of ovaries, where rDNA is highly transcribed. In this cell type, Xnp localizes broadly in the nucleus but not within the nucleolus, but most Hira protein forms foci within the nucleolus. A pulse of epitope-tagged H3.3 produced in follicle cells broadly labels the nucleus and foci within the nucleolus, corresponding to transcriptionally active sites in this cell type. Follicle cells from xnp mutant ovaries also show nucleolar labeling with H3.3-GFP, demonstrating that Xnp is not required for nucleolar RI assembly. In contrast, a pulse of epitope-tagged H3.3 in Hira mutant follicle cells does not deposit in the nucleolus. Thus, rDNA chromatin must rely on the Hira chaperone for H3.3 deposition. It is concluded that Xnp and Hira are redundant at many sites within the genome, but some sites rely on individual factors for replacement nucleosome assembly. Although neither Hira nor Xnp are individually required for viability, there may be more subtle phenotypes that occur in repetitive sites in the genome (Schneiderman, 2012).
If Xnp and Hira are generally involved in recognizing chromatin gaps, the localization of these factors should be affected in H3.3-deficient cells. Indeed, new binding sites for Xnp appear in rDNA chromatin after H3.3 knock-down. Hira is also recruited to the nucleosome-depleted satellite block after H3.3 knock-down. Strikingly, the area of the nucleosome-depleted satellite block is ∼2.5-times larger after H3.3 knock-down, and the Xnp signal at this site is elevated. This finding implies that RI assembly is normally required for compaction of the satellite. The redundancy of Hira and Xnp implies that their importance for H3.3 deposition is underestimated in single-mutants. Both the relocalization and increased binding of Xnp and Hira after H3.3 knock-down support the idea that these assembly factors are recruited to aberrant, nucleosome-depleted chromatin. As persistent exposure of DNA may disrupt transcriptional regulation or allow DNA damage, surveying chromatin for gaps with RI assembly factors may be critical for genome stability and function (Schneiderman, 2012).
Histone variants are non-allelic isoforms of canonical histones and they are deposited, in contrast to canonical histones, in a replication-independent (RI) manner. RI deposition of H3.3, a histone variant from the H3.3 family, is mediated in mammals by distinct pathways involving either the histone regulator A (HIRA) complex or the death-associated protein (DAXX)/alpha-thalassemia X-linked mental retardation protein (ATRX) complex. This study investigated the function of Drosophila DAXX Like Protein (DLP) by using both fly genetics approaches and protein biochemistry. DLP specifically interacts with H3.3 and shows a prominent localization on the base of the X chromosome, where it appears to act in concert with XNP the Drosophila homolog of ATRX, in heterochromatin assembly and maintenance. The functional association between DLP and XNP is further supported by a series of experiments, which illustrate genetic interactions and DLP-XNP-dependent localization of specific chromosomal proteins. In addition, DLP both participates in RI deposition of H3.3 and associates with the anti-silencing factor-1 (ASF1). It is suggested, in agreement with a recently proposed model, that DLP and ASF1 are part of a pre-deposition complex, which is recruited by XNP and is necessary to prevent DNA exposure in the nucleus (Fromental-Ramain, 2017).
This study has identified DLP as the Drosophila homolog of DAXX. DLP is involved, likely in concert with XNP/dATRX, in the formation of pericentric heterochomatin of the X chromosome. Moreover, DLP is implicated in RI deposition of the histone variant H3.3 and may constitute with ASF1 the central core of a pre-deposition complex, recruited to chromatin gaps by XNP. The existence of such complex was recently suggested (Fromental-Ramain, 2017 and references therein).
In spite of the fact that both proteins do not molecularly associate as their mammal homologs do, this study provides evidence that DLP and XNP functions are closely linked. DLP and XNP are located on the base of the X chromosome and analysis of animals simultaneously mutant for both dlp and xnp revealed that DLP and XNP likely act together during heterochromatin formation. In addition, both DLP and XNP are located next to distal heterochromatic marker HP1 on the X chromosome of larvae carrying the ln(1)wm4h rearrangement. Functional interactions between DLP and XNP 55 were also supported by the similar behavior of DLP and XNP in H3.3 deficient cells. In wild-type cells, in addition to the base of the X chromosome, expression of XNP is detected at many sites across the chromosome arms where DLP is not observed. In H3.3 knock-down-cells, DLP and XNP are present at many euchromatic sites of the chromosomes and are simultaneously associated with nucleolar chromatin of the rDNA. Finally, overexpressed DLP binds to many interbands on the polytene chromosomes, suggesting that DLP may also be involved in chromatin organization at euchromatic sites in addition to the pericentric heterochromatin. However, this latter observation should be viewed with caution since it cannot be ruled out that over-expressed DLP is not present in its usual complex and is consequently mis-targeted. Additional support for functional interactions between XNP and DLP is provided by genetic interactions between xnp and dlp. Indeed, loss of xnp function is characterized by reduced viability, which is further aggravated when dlp function is simultaneously reduced, strongly indicating that xnp and dlp may functionally cooperate during regulation of common targets. How XNP is recruited to nucleosome-depleted chromatin remains an important issue. XNP may be recruited by transcriptional machinery to active genes. Alternatively, XNP may bind structural motifs common to chromatin gaps, or may simply bind exposed DNA. The homologous ATRX contains a PHD domain that can bind DNA or histones tails. Recent work demonstrates that mammalian Hira may bind exposed DNA at chromatin gaps. Moreover, Hira and XNP bind active regions independently of one another. Hence, there may be multiple ways that RI assembly factors recognize exposed DNA (Fromental-Ramain, 2017).
In Drosophila, loss of H3.3 has a large impact on viability and fertility of both males and females. The Drosophila genome encompasses two single copy genes, H3.3A and H3.3B, which code for the same protein. H3.3 is highly expressed in mitotic, meiotic and post-meiotic male germ cells, probably reflecting high transcriptional activity. Interestingly, high dlp expression is observed in primary spermatocytes, in meiotic spermatocytes and also in the germinal vesicle, suggesting that it may have important functions during development of germ cells. In Drosophila testis, H3.3 disappears with the bulk of histones, prior to accumulation of protamine and other sperm-specific nuclear basic proteins, leading to sperm DNA compaction at late stages of spermiogenesis. At fertilization, assembly of nucleosomes on paternal DNA immediately follows the rapid loss of protamines from the decondensing male nucleus and is dependent on maternally provided factors like Hira and YEM. HIRA and YEM are crucial since male pronuclei fail to decondense at the pronuclear stage in eggs derived from female mutants for HIRA and YEM. Hence, function of HIRA/YEM at fertilization represents a unique example where deficient chromatin activity cannot be compensated by other redundant factors (Fromental-Ramain, 2017).
In contrast, many examples suggest that H3.3 chaperones/chromatin remodeling complexes may display functional redundancy as mutants in these factors have limited phenotypes. In this context, DLP may be viewed as a typical example. The null allele dlpG and the dlp45 allele encoding a truncated protein lacking the C-terminal DHR necessary for H3.3 binding are viable and fertile, indicating that DLP and other chromatin factors may share common functions. Alternatively, DLP may display accessory functions during development of germ cells. Characterization of the phenotypes of double-mutant animals during germ cell development would help to resolve this important issue (Fromental-Ramain, 2017).
H3.3 was initially seen as a characteristic of active genes with histone turnover occurring as a consequence of transcription. More recent studies revealed that H3.3 is widespread within the genome. In particular, H3.3 is deposited by ATRX/DAXX at telomeres and pericentric repeats. Interestingly, ATRX and DAXX are components of the same chromatin-remodeling complex and physically interact. Recently, Schneiderman (2012) proposed a model on how XNP, the Drosophila homolog of ATRX, and HIRA identify nucleosome-depleted DNA following gene activation, and promote nucleosome assembly through a three steps process. Initially, XNP and HIRA bind exposed DNA at chromatin gaps where nucleosomes have been displaced. Subsequently they co-operate to recruit a predeposition complex including ASF1 and histones. In the final step, XNP and HIRA assist the transfer of histones from delivery factors to DNA and are released when nucleosome assembly is complete. Even if XNP and DLP do not physically interact, this study provides several evidences suggesting that DLP could be a component of the predeposition complex recruited by XNP/HIRA (Fromental-Ramain, 2017).
Both HIRA and XNP have been implicated in RI nucleosome assembly, but mutants of these factors have only limited phenotypes, revealing that they have redundant functions. Thus, single mutants of either xnp or hira weakly affect H3.3 deposition, which is abolished in a double-mutant of xnp and hira. This observation highlights the need for two distinct pathways during RI nucleosome assembly, one mediated by HIRA/YEM and the other by XNP. This study assigns a role to DLP during RI H3.3 deposition since H3.3 incorporation is affected in animals lacking DLP. DLP is thought to co-operate with XNP and it was surprising to observe H3.3 deposition in animals lacking HIRA and DLP. Hence, it is speculated that the pathway mediated by XNP is always functional, although less efficient. It has been recently proposed that XNP recognizes exposed DNA when a nucleosome has been displaced, and serves as a binding platform for the recruitment of H3.3 predeposition complexes to chromatin gaps. Such complexes are believed to contain (H3.3-H4) heterodimers, ASF1 and additional factors. In line with this the data revealed physical interactions between ASF1 and DLP in protein extracts made from baculovirus-infected Sf9 cells co-expressing DLP and ASF1, suggesting that DLP may be one of these additional factors (Fromental-Ramain, 2017).
These data provides additional links between HIRA, DLP, ASF1 and XNP during H3.3 incorporation but how they functionally interact during development remains an open question. Identification of their genomic targets and characterization of their activities during H3.3 deposition would obviously help to resolve this important issue (Fromental-Ramain, 2017).
The histone H3 family contains an evolutionary conserved variant, H3.3, that differs in sequence in only five amino acids from the canonical H3. There are four differences between Drosophila H3 and H3.3.
date revised: 6 August 2005
Home page: The Interactive Fly
© 1995, 1996 Thomas B. Brody, Ph.D.
The Interactive Fly resides on the
Society for Developmental Biology's Web server.