|Mutation Type||critical splice donor site (2 bp from exon)|
|Coordinate||45,431,318 bp (GRCm38)|
|Base Change||A ⇒ T (forward strand)|
|Gene Name||RuvB-like protein 2|
|Chromosomal Location||45,421,852-45,438,096 bp (-)|
|MGI Phenotype||Mice homozygous for an ENU-induced allele exhibit lethality. Mice heterozygous for a knock-out allele exhibit impaired T cell development and maximal T dependent antibody responses.|
|Amino Acid Change|
|Institutional Source||Beutler Lab|
Ensembl: ENSMUSP00000033087 (fasta)
Ensembl: ENSMUSP00000103400 (fasta)
|Gene Model||not available|
|Phenotypic Category||decrease in CD4+ T cells, T-dependent humoral response defect- decreased antibody response to rSFV|
|Alleles Listed at MGI|
|Mode of Inheritance||Autosomal Dominant|
|Local Stock||Live Mice, Sperm|
|Last Updated||05/13/2016 3:09 PM by Stephen Lyon|
|Record Created||03/09/2010 2:11 PM by Carrie N. Arnold|
|Other Mutations in This Stock||
Stock #: G4846 Run Code: SLD00228
Coding Region Coverage: 1x: 77.7% 3x: 53.3%
Validation Efficiency: 104/115
The index Worker mouse was identified among the ENU-mutagenized G3 population. It displayed suboptimal T-dependent IgG responses to recombinant Semliki Forest Virus (rSFV)-encoded β-galactosidase in the T-dependent humoral response screen (Figure 1, right), and normal T-independent IgM responses to NP-Ficoll (T-independent B cell response screen) (Figure 1, left) (1).
When Worker mice were injected with NP-CGG, seven days post-immunization the mice were found to have undetectable levels of NP-specific IgM (Figure 3A) and low levels of NP-specific IgG1 (Figure 3B) (1), consistent with an impaired extrafollicular response in these mice. At day 14 post-immunization, the Worker IgG1 and IgM responses were normal; at 28 days post-immunization, most of the NP-specific IgG1 was high affinity (Figure 3C), indicating that affinity maturation occurs in Worker mice (1). Memory B cell function was normal in Worker mice.
The humoral response and T cell deficiencies of Worker mice were dominant but incompletely penetrant (one third of heterozygotes displayed these phenotypes), and fully concordant with white belly spotting. Expressivity of the pigmentation phenotype varies, ranging from a few white hairs to large patches covering the abdomen (Figure 4). Homozygosity for the Worker mutation causes lethality at an undetermined prenatal stage.
|Nature of Mutation|
The dominant Worker mutation was mapped by bulk segregation analysis (BSA) of F1 offspring (n=9 with mutant phenotype, 63 with normal phenotype) of Worker males crossed to C57BL/10J females. Strongest linkage was observed with the marker at position 71519895 bp on chromosome 7 (synthetic LOD=10.7), within a critical region of 54410823 - 87465557 bp. However, separate sample genotyping revealed that the T-dependent IgG response phenotype is not fully penetrant, and defined the critical region as 38216957-71519895 bp, with strongest linkage to the marker at 54410823 bp (LOD=5.02). Whole genome SOLiD sequencing of a Worker mutant identified a T to A transversion at position 3147 of the genomic sequence of Ruvbl2 (NC_000073), affecting the second nucleotide of intron 2. Ruvbl2 contains 15 exons (ENSMUST00000107771).
The Worker mutation causes skipping of exon 2, resulting in a frameshift upon splicing of exon 1 to exon 3, as shown below. A premature stop codon following 27 aberrant amino acids encoded by exon 3 and part of exon 4 is expected to cause nonsense-mediated decay of the transcript. However, the incomplete penetrance of the Worker phenotype among heterozygous mice suggests that in some animals at least some normal splicing may occur; thymic cDNA sequencing confirmed this hypothesis.
<--exon 1 exon 2 intron 2--> exon 3--> 202 ATGGCAACCGTG GCAGCCACC……GAGCGAATCG GTGAGTGAGCA GCGCTCACTCCCACATCCGGGGGCTGGGACTGGATG..GGCAGCTAG 1 -M--A--T--V- -A--A--T-……-E--R--I-- -A--L--T--P--T--S--G--G--W--D--W--M-..-G--S--*- correct deleted aberrant
The mutated nucleotide is indicated in red lettering; the splice donor site is in blue. Nucleotide numbering corresponds to the genomic NCBI reference sequence (NC_000073).
Ruvbl1 and Ruvbl2 are paralogous ATPases of the AAA+ (ATPases associated with diverse cellular activities) superfamily, the members of which are structurally similar but functionally diverse. All AAA+ proteins contain a structurally conserved ATP-binding module that hetero- or homo-oligomerizes into active complexes, most commonly hexamers (2). AAA+ proteins switch between at least two distinct nucleotide-mediated conformational states, transducing these conformational changes to target molecules. Intersubunit interactions within oligomers, for example through a characteristic ‘arginine-finger’ (3;4), enable conformational changes to be propagated from one active site to the next. Thus, depending on the kinetics of nucleotide binding and release, AAA+ oligomers can function as bimodal switches or processive motors.
Ruvbl1 was identified in rat liver nuclear extracts in a complex containing TATA-binding protein (TBP) (5) and shown to possess ATPase activity that was stimulated by single-stranded DNA, but not RNA or double-stranded DNA (6). Ruvbl2 was discovered as a Ruvbl1-related protein (42% identical) by sequence analysis of the Saccharomyces cerevisiae genome (7;8), and was subsequently cloned from a human liver cDNA library (9). Ruvbl2 also displayed single-stranded DNA-stimulated ATPase activity. Ruvbl1 and Ruvbl2 share sequence similarity with the bacterial protein RuvB, a helicase with 5’ to 3’ DNA unwinding activity required for DNA repair and recombination. Together with bacterial RuvA, RuvB binds to the four-stranded DNA crossover intermediate known as the Holliday junction and promotes branch migration in an ATP-dependent manner (10;11). Both Ruvbl1 and Ruvbl2 display ATP-dependent DNA helicase activity in vitro (9). The directionality of Ruvbl2 helicase activity has been reported to be 3’ to 5’ (9). For Ruvbl1, both 5’ to 3’ (9) and 3’ to 5’ (6) helicase activities have been reported; other groups failed to detect helicase activity at all (8;12;13).
Ruvbl2 shares the same domain organization (Figure 5) and presumably the same overall 3D structure as Ruvbl1. The X-ray crystal structure of monomeric ADP-bound human Ruvbl1 revealed the canonical AAA+ domain fold consisting of a nucleotide-binding core domain made from a five-stranded β sheet sandwiched between two α helices (αβα domain), and a bundle of four α helices that caps the nucleotide-binding pocket (Figure 6, PDB ID 2C90) (12). The αβα nucleotide-binding domain contains a Walker A motif (GXXXXGK[T/S]) important for binding and orienting ATP, a Walker B motif (hhhhDEX[H/N], h=hydrophobic) required for ATP hydrolysis, and sensor-I and sensor-II elements that discriminate between di- and triphosphate nucleotides. The αβα domain is interrupted by an ‘insertion domain’ of 170 amino acids between the Walker A and Walker B motifs; such an insertion is not found in RuvB or in most other AAA+ proteins (Figure 5) (8;9;12). The insertion domain resembles the DNA-binding domain of replication protein A (RPA; required for DNA recombination, repair and replication), and by itself can bind to ssDNA, dsDNA, and ssRNA (12).
In the crystal structure, Ruvbl1 assembles into a hexameric structure with a central channel (12). The central channel has a diameter of 18 Å, which is sufficient for ssDNA but not dsDNA to pass through. Negative electrostatic potential of the channel also favors interaction with ssDNA over dsDNA. The authors proposed that one strand of a forked DNA substrate is threaded through the channel, while the second strand binds to the outside of the ring through an interaction with the insertion domain. Nucleotide binding occurs at the interface between subunits, but hexamerization results in inaccessibility of the nucleotide-binding pocket and inability to exchange ATP for ADP. No ATPase activity, and consequently no helicase activity, was observed for this structure. It was proposed that a conformational change is required for successful completion of nucleotide hydrolysis and release. Arginine 357 serves as the ‘arginine-finger’ described above, forming part of the nucleotide binding pocket of the adjacent subunit, and suggesting that intersubunit cooperativity contributes to Ruvbl1 function.
Ruvbl1 and Ruvbl2 interact as purified proteins and in yeast two-hybrid experiments, and co-immunoprecipitate in a large complex from HeLa nuclear extracts (9). Three rather different electron microscopic structures of Ruvbl1 and Ruvbl2 heterohexamers have been reported [(14-16); discussed in (17)], highlighting the fact that the in vivo oligomeric state of these proteins remains unknown. The human Ruvbl1-Ruvbl2 complex is an asymmetric double hexameric ring with a central channel 26 Å in diameter, large enough to accommodate dsDNA (16). Similarly, the yeast Ruvbl1-Ruvbl2 complex examined by cryo-electron microscopy (EM) is organized into an asymmetric double hexameric ring with a 25 Å diameter (14). In this structure, electron density was observed sandwiched between the top and bottom rings and was proposed to derive from intercalating insertion domains at the equator of the structure. Contrasting with these structures is the yeast Ruvbl1-Ruvbl2 complex visualized by negative-staining scanning transmission EM, which forms a single hexameric ring that changes conformation upon binding to ATP or ADP (15). In none of these three structures were the identities of individual subunits discernable. Thus, whether the single rings were homomeric or heteromeric, and whether the double hexamers were formed from stacks of homomeric or heteromeric rings could not be determined.
The single and double hexameric structures may represent different functional states of Ruvbl1-Ruvbl2 complexes, but it has also been suggested that the double hexameric structure is an artifact induced by histidine tags (18), which were employed in the studies by Puri et al. (16) and Torreira et al. (14). Another study used size-exclusion chromatography, analytical ultracentrifugation, and mass spectrometry to investigate the different oligomeric forms of human Ruvbl1-Ruvbl2 complexes (19). Ligand-free Ruvbl1 and Ruvbl2 were shown to be monomeric; Ruvbl2 formed hexamers in the presence of nucleotide. When co-expressed and purified from E. coli, Ruvbl1-Ruvbl2 complexes comprised monomeric, dimeric, trimeric, hexameric and dodecameric species. Mass spectrometry of the hexamers demonstrated that the complexes contained Ruvbl1 and Ruvbl2 mixed in various stoichiometries. Ruvbl1 and Ruvbl2 exist in multiple protein complexes in cells, and their oligomeric states in vivo remain to be determined.
A recent study crystallized the biologically active human Ruvbl1/Ruvbl2 complex at 3Å resolution [PDB: 2XSZ; (20); Figure 7]. The crystal consists of truncated Ruvbl1 and Ruvbl2 proteins (Ruvbl1 is missing aa 127-233; Ruvbl2 is missing aa 134-237); a linker was inserted to replace the deleted regions. The complex is comprised of two heterohexamers stacked on each other to form a dodecamer. This study determined that the hexameric ring is composed of alternating Ruvbl1 and Ruvbl2 monomers. The nucleotide-binding pockets of each heterohexamer are close to the top and bottom faces of the dodecamer at the interface between the AAA+ domain (αβα) and the AAA+ domain (α); the hexameric rings interact through the retained, internal region of the insertion domain. The findings in this study indicated that ATP hydrolysis activity was 3 times higher in the complex relative to the individual wild type Ruvbl1 and Ruvbl2 proteins, consistent with previous studies (13-16). A complex of the truncated versions of Ruvbl1 and Ruvbl2 used for crystallization displayed even higher ATPase activity. The truncated proteins individually also displayed 2-fold higher ATPase activity compared to the individual wild type proteins. In agreement with previous reports that wild type purified Ruvbl1 and Ruvbl2 lacked helicase activity (8;12;13), only the truncated forms of Ruvbl1 and Ruvbl2, either individually or in complex, showed helicase activity toward a dsDNA substrate (20). Gorynia et al. thus propose that the DNA helicase activity of Ruvbl1 and Ruvbl2 can be autoinhibited by the insertion domain and that cofactors within chromatin remodeling complexes may bind to the proteins, causing a conformational change to the insertion domain that permits subsequent helicase activity (20). Measurements of the central channel of the dodecamer indicate that it is 85 Å long and has an ~19 Å internal diameter at either end, respectively. The central part of the channel is much wider (~35 Å). Gorynia et al. report that the crystal structure of the Ruvbl1-Ruvbl2 complex differs from the EM studies mentioned above. For example, the crystal structure is symmetrical as opposed to the findings of Puri et al. (16) and Torreira et al. (14). Second, the crystal structure shows a heterohexameric arrangement of monomers within a dodecamer (as opposed to the isolated hexamers proposed by Gribun et al. (15)).
Western blot analysis revealed that Ruvbl2 was most abundantly expressed in thymus and testis (9), whereas Ruvbl1 was most abundantly expressed in spleen, thymus, lung, and testis (6;21). Data from the BioGPS database supports strong expression in testis in both mice and humans, and moderate expression in the thymus (~3X the median in humans) and thymocytes (roughly equivalent to the median in mice) (see figure 8). In mouse follicular B cells, bone marrow macrophages, and whole bone marrow, Ruvbl2 transcript levels are approximately 3X the median level.
The circumstances in which Ruvbl1 and Ruvbl2 were discovered suggested their intimate involvement with DNA and/or with the machinery that regulates DNA. For example, the findings that they interacted with TBP (5;9) and were components of the RNA polymerase II holoenzyme (8) suggested a role in transcription. The association of Ruvbl1 with RPA (8), and the homology between bacterial RuvB and both Ruvbl1 and Ruvbl2 led to the hypothesis that the Ruvbl proteins play a role in DNA replication or recombination. More recent discoveries have demonstrated that Ruvbl1 and Ruvbl2 participate in chromatin remodeling during the processes of transcription, DNA damage repair, and DNA replication; and aid in the assembly and stabilization of ribonucleoprotein complexes.
Despite the abundance of in vitro data, the function(s) of Ruvbl1 and Ruvbl2 in whole organisms and the physiological processes requiring them remain largely unknown. Studies using S. cerevisiae have shown that both Rvb1 and Rvb2 (as they are known in yeast) are essential genes (8;9). The ATP binding and hydrolysis activity of Rvb1 and Rvb2 are also required for the viability of yeast (24). Yeast with conditional mutations in either Rvb1 or Rvb2 displayed rapid changes, both upregulation and downregulation, in the transcription of over 5% of the yeast genome upon shift to the non-permissive temperature. However, whether helicase activity is important in vivo has not been shown. To date, no mouse model of Ruvbl1 or Ruvbl2 deficiency has been reported.
Nucleosomes consist of a histone octamer (two each of H2A, H2B, H3, and H4) and 147 base pairs of DNA wrapped two times around it (Figure 9). Chromosomal DNA is packaged into nucleosomes to facilitate its compact packing into the nucleus, but nucleosomes must be disassembled in order to gain access to DNA for transcription, replication, or repair. The process of nucleosome assembly and disassembly is controlled by several chromatin remodeling complexes that use the energy of ATP to slide nucleosomes along DNA, to remove histones and nucleosomes, or to replace canonical histones with histone variants, which induce distinct chromatin structures that signal particular DNA processing events such as transcription or repair. Histones are further regulated by histone acetyltransferases (HATs) and deacetylases (HDACs) that promote either relaxation or tightening, respectively, of the association of DNA with the modified histones.
Ruvbl1 and Ruvbl2 have been identified as members of the mammalian INO80 (named for an inositol-requiring S. cerevisiae strain containing a mutation in Ino80) and SRCAP (Snf2-related CREB-binding protein activator protein) complexes that mediate nucleosome remodeling, and as a member of the Tip60 HAT complex (Figure 10). These three complexes share at least one subunit, actin regulatory protein 4 (Arp4), which has been shown to bind directly to histones (25-27). Each complex functions in a mechanistically distinct way to remodel chromatin.
INO80 and SWR1 complexes
All known ATP-dependent chromatin remodeling complexes contain a SNF2 family ATPase that is responsible for the nucleosome remodeling activity of the complex. Ino80 is a member of the SNF2 family of chromatin remodeling proteins, and functions in a complex containing approximately fifteen proteins including Ruvbl1 and Ruvbl2. The INO80 complex was first identified in yeast (28;29), and a similar human complex containing eight orthologous proteins along with seven human-specific proteins has also been identified (30). The core subunits common to yeast and humans are Ruvbl1 and Ruvbl2, present in 6:1 stoichiometry relative to other subunits, as well as Ino80, Arp4, Arp5, Arp8, Ies2, and Ies6 proteins. In yeast, acute inactivation of Ino80 or Rvb2 affected significantly overlapping sets of genes (31). Based on the finding that INO80 complexes isolated from Rvb2-deficient yeast lacked Arp5 and Rvb proteins, it has been hypothesized that the Rvb proteins are required for the assembly of Arp5p into the complex (31). Indeed, studies examining other Ruvbl protein-containing complexes suggest that an important function of these AAA+ ATPases is facilitating the assembly of complexes, possibly by acting as scaffolding proteins.
The yeast chromatin remodeling complex SWR1 (named for S. cerevisiae strain ‘Sick With Rat8 ts’ that contains a mutation in Swr1, and known as SRCAP in mammals) consists of fourteen subunits (10 in mammals) including the SNF2 family ATPase Swr1, Rvb1, and Rvb2 (32-34). Between the yeast and human complex six subunits are conserved: Swr1, Rvb1, Rvb2, Arp4, Arp6, and Yaf9 (yeast names given). Like INO80, the SWR1 complex exhibits nucleosome-stimulated ATPase activity. In the yeast complex, the Rvb proteins associate with the ATPase domain of Swr1, which is also required for the association of four other subunits. This finding suggests that Rvb proteins may aid in the assembly of the SWR1 complex. However, a function for Rvb proteins in the assembled SWR1 complex is unknown.
-Regulation of transcription
Both INO80 and SWR1 complexes help to regulate transcription, but do so using different mechanisms. The INO80 complex functions to reposition (‘slide’) nucleosomes along the DNA (25;35), and to completely remove nucleosomes from the DNA (36;37). INO80 complexes lacking Rvb1 and Rvb2 failed to reposition nucleosomes in a 12-nucleosome model substrate (31). In mammalian cells, the transcription factor YY1, itself an INO80 complex component, is required to recruit the INO80 complex to target promoters (38). Paradoxically, the INO80 complex is also required for binding of YY1 to target genes. It was suggested that the INO80 complex moves or removes promoter-associated nucleosomes in order to enable YY1 to gain access to its targets.
The SWR1 complex facilitates ATP-dependent replacement of canonical histone H2A with the variant H2AZ in the nucleosome (32-34). Chromatin containing H2AZ adopts a distinct conformation compared to H2A-containing chromatin, and is typically associated with transcriptionally active chromatin (39;40), although it may also help to establish heterochromatin under specific contexts (41;42).
-DNA damage responses
Eukaryotic cells repair DNA double strand breaks (DSBs) by both non-homologous end joining (NHEJ) and homologous recombination. Upon sustaining a DSB, DNA ends are recognized and bound by the MRN (Mre11-Rad50-Nbs1) complex (known as the MRX complex in yeast), which promotes the production of single stranded 3’ overhangs in a process called resection. These single stranded DNA regions recruit the kinases ATM (ataxia telangiectasia mutated) and ATR (ataxia telangiectasia and Rad3 related), which both phosphorylate histone variant H2AX and activate the checkpoint kinases Chk1 and Chk2. Phosphorylation of H2AX spreads over megabases surrounding the DSB site, and is required for stable accumulation of repair proteins. In particular, INO80 and SWR1 complexes bind directly to DSBs through association with phospho-H2AX (43;44).
Both INO80 and SWR1 complexes are required for processing broken DNA ends, and perform different functions. INO80 promotes eviction of proximal nucleosomes surrounding DSBs, including nucleosomes containing phospho-H2AX and H2AZ (36;37;45). Nucleosome eviction facilitates the association of other repair proteins to the DSB, and the invasion of the single stranded DNA into the homologous donor locus. In contrast, SWR1 is required for recruitment to DSB regions of Mec1 (the yeast ATR-related kinase) and Ku80, proteins required for NHEJ (36;46). Mutations of the Arp subunits of the yeast INO80 complex lead to defects in both homologous recombination and NHEJ, whereas mutations of Swr1 affect the NHEJ pathway.
DNA repair is closely tied to the activation of cell cycle checkpoints that allow time for repair of damaged DNA followed by re-entry into the cell cycle. Mutations in INO80 and SWR1 complex subunits result in delayed checkpoint activation (36;46), although the mechanisms by which the complexes influence checkpoint regulation are not known. A possible clue is that the Ies4 subunit of the INO80 complex is phosphorylated by Mec1 and Tel1 (the yeast ATR and ATM proteins) during exposure to DNA damaging agents (47).
The yeast INO80 complex is enriched at DNA replication origins, even more abundantly at stalled replications forks that are under replicative stress (48-50). Mutation of Ino80 results in dissociation of components of the replication machinery from the replication fork, leading to defects in sustained replication and survival of yeast exposed to agents that cause replication fork stalling (50). The human INO80 complex has also been shown to participate in DNA replication, binding to replication forks during S phase of the cell cycle (51).
The TIP60 complex (named for HIV Tat interactive protein 60 that was originally identified as an activator of Tat-dependent transcription) acetylates the ε-amino groups of lysine residues on nucleosomal histones H2A and H4, as well as on other cellular proteins (52). Proteins of the mammalian TIP60 complex are orthologous to proteins in either the NuA4 (nucleosomal acetyltransferase of H4) or the SWR1 complexes of yeast (13;53). Thus, Ruvbl1 and Ruvbl2, which are part of the TIP60 complex and required for its histone acetyltransferase activity (54), are found in the SWR1 complex but not in the NuA4 complex. It has been proposed that the functions of the two yeast complexes have been integrated into a single complex in mammals (53).
The TIP60 complex interacts with a variety of proteins that target the complex to specific substrates. To promote transcription, it is recruited by a number of transcription factors to acetylate histones at promoters. For example, c-Myc has been shown to induce histone H4 acetylation at its target promoters by recruiting the TIP60 complex, including Ruvbl1 and Ruvbl2 (55). The transcriptional activator E2F1 also binds to and recruits the TIP60 complex to its target promoters to induce histone acetylation (56). Transcriptional activation of histone genes has been shown to require recruitment of the TIP60 complex to histone promoters during the G1/S transition (57).
In addition to transcriptional regulation, the TIP60 complex plays a key role in DSB repair by both influencing chromatin remodeling at DSBs, and by acetylation and activation of the ATM kinase. The TIP60 complex is recruited to DSBs by phosphorylated H2AX similarly to the INO80 and SWR1 complexes (27). TIP60-mediated acetylation of H2AX and H4 at DSBs promotes the recruitment of repair proteins and its absence results in defective repair by homologous recombination (13;58). In addition, acetylation of histone H4 by TIP60 is required for the exchange of phospho-H2AX, which marks the damaged region of DNA, for unmodified H2AX (59;60). Another group reported that TIP60 acetylation of histone H4 is required prior to the dephosphorylation of phospho-H2AX surrounding the DSB (54).
The TIP60 complex also acetylates ATM in response to DNA damage, a modification that contributes to activation of ATM kinase activity (61;62). However, it was also reported that downregulation of Ruvbl1 does not reduce phosphorylation levels of ATM substrates (54).
Assembly and stabilization of protein complexes
Small nucleolar RNAs (snoRNAs) function within protein-containing complexes called small nucleolar ribonucleoproteins (snoRNPs) that modify and process other noncoding RNAs including small nuclear RNA (snRNA), tRNA, and most commonly, ribosomal RNA (rRNA) (Figure 11). The snoRNAs, like other noncoding RNAs, function as adaptors that guide substrate RNAs via Watson-Crick base pairing to the active site of the RNP. They are divided into two classes based on the nucleotide modifications they guide. Box C/D snoRNAs direct 2’-O-ribose methylation, and box H/ACA snoRNAs guide pseudouridylation (isomerization of uridine to pseudouridine). These modifications are required for ribosome and spliceosome function.
snoRNAs interact with core sets of highly conserved proteins to form the box C/D and H/ACA RNPs. These proteins are cotranscriptionally assembled with the nascent RNA to form a stable snoRNP, and Ruvbl1 and Ruvbl2 are thought to be required for this process, which occurs in the nucleoplasm. When Rvb2 was depleted from yeast, box C/D and box H/ACA snoRNA levels were reduced and core proteins of both snoRNPs were mislocalized from the nucleolus to the nucleoplasm (23). Mutation of the box C/D motif of the U14 snoRNA prevented binding of C/D core proteins as well as binding of Ruvbl1 and Ruvbl2, and resulted in mislocalization of the snoRNA from the nucleolus to the nucleoplasm (63). These findings suggested that Ruvbl1 and Ruvbl2 are assembly factors, perhaps acting as scaffolding proteins for snoRNPs. A restructuring event that stabilizes the interactions of the core proteins with the snoRNA has been shown to occur during snoRNP maturation (64). The interaction of Ruvbl1 and Ruvbl2 with multiple core box C/D proteins led to the hypothesis that, in addition to aiding snoRNP assembly, Ruvbl1 and Ruvbl2 mediate this restructuring event (22;64-66).
Phosphatidylinositol 3-kinase-related kinase (PIKK) proteins
In yeast, Rvb1 and Rvb2, together with Tah1 and Pih1 (also called Nop17), form the R2TP complex that associates with the chaperones Hsp90 (67;68) and prefoldin proteins (69). The subcellular localization of the interactions between R2TP and either Hsp90, prefoldin 2, or prefoldin 6 is unknown, since these interactions were identified using immunoprecipitation or affinity purification from soluble fractions of whole cell lysates. The mammalian R2TP complex has been proposed to itself act as a cytoplasmic chaperone that stabilizes members of the PIKK family that includes ATM, ATR, DNA-PKcs, mTOR, SMG1, and TRRAP (70). Ruvbl1 and Ruvbl2 associated with all PIKKs in pull down assays, and knockdown of either Ruvbl1 or Ruvbl2 in HCT116 colorectal carcinoma cells led to an impairment of PIKK-mediated signaling, for example Chk1 and Chk2 phosphorylation in response to DNA damage (74). In addition, Ruvbl1 and Ruvbl2 regulate the abundance of PIKK mRNAs, possibly by regulating their transcription as part of chromatin-remodeling complexes or in conjunction with transcription factors (56;71;72). The R2TP complex is also believed to contribute to snoRNP biogenesis and snoRNA accumulation (67;68;73;74).
Telomerase core complex
The telomerase complex adds telomere repeats to the ends of chromosomes, and is another RNP complex reported to require Ruvbl1 and Ruvbl2 for proper assembly (75). Telomerase reverse transcriptase (TERT), the telomerase RNA component (TERC), and the TERC-binding protein dyskerin are the three essential components of the complex. Ruvbl1 interacts directly with TERT and dyskerin, and depletion of Ruvbl1 and Ruvbl2 results in reduced telomerase complex accumulation.
The Worker mutation likely causes nonsense-mediated decay of the Ruvbl2 transcript. Homozygous mutation causes lethality, whereas heterozygous mutation causes a humoral immune phenotype in one-third of heterozygous mice. Following are several hypotheses for the mechanism of the Worker mutation.
The white belly spotting observed in Worker mice is indicative of defective melanoblast migration during embryogenesis. The incomplete penetrance and perfect concordance of immune and pigmentation phenotypes in Worker mice suggest the possibility of an epigenetic mechanism of the mutation, which may exert its effects during embryogenesis. The consequences are observed in distinct cell types that differentiate long afterward: T cells (derived from hematopoietic stem cell precursors of the yolk sac) and melanocytes (derived from the neural crest). The involvement of Ruvbl2 in the regulation of chromatin remodeling by the INO80, SRCAP, and TIP60 complexes supports this hypothesis.
Reduced T-dependent IgG responses were observed in heterozygous Worker mice. The underlying defect appears to be T cell-dependent, since B cell responses to T-independent antigens and B cell development were observed to be normal. Moreover, CD4+ and CD8+ T cells were reduced in the mutant mice. These data are consistent with the relatively high expression of Ruvbl2 in the thymus and in thymocytes, which suggests a T cell-intrinsic effect of the Worker mutation. The existence of Ruvbl1 and Ruvbl2 in the INO80, SRCAP, and TIP60 complexes, all of which participate in the repair of DNA double strand breaks, raises the possibility that they contribute to double strand break repair during V(D)J recombination. Impaired repair of DSBs made by RAG1/RAG2 during V(D)J recombination in thymocytes, but not in immature B cells, might ultimately result in reduced numbers of T cells in Worker mice. In support of this hypothesis, homozygous null and nonsense mutations in the NHEJ DNA repair factor DNA-PKcs cause T cell-negative, B-cell negative severe combined immunodeficiency (SCID) (76), and a missense mutation causes a decrease in lymphocyte numbers (Prkdchanky; MGI: 4820716). Mutations in other components of the NHEJ machinery, including Lig4 (77) and Artemis (78), result in impaired V(D)J recombination and various degrees of B and T lymphocyte reduction, most more severe than observed in Worker mice.
As in Worker mice, immune and pigmentation phenotypes together with putative impairment of RNP function are observed in the syndrome dyskeratosis congenita (OMIM #127550, #305000, #224230). The disease is characterized by nail dystrophy, skin hyperpigmentation, and oral leukoplakia, as well as immunodeficiency and bone marrow failure. A report indicates that immunological abnormalities (lymphopenia, low B-cell numbers, hypogammaglobulinemia, and decreased T-cell function) were the most frequent laboratory findings at initial presentation (79). The disease is caused by premature telomere shortening leading to death of high-turnover cell types including hematopoietic cells, immune cells, and epithelial cells. Mutations in one of at least five genes encoding dyskerin (X-linked), TERC (autosomal dominant disease), TERT (autosomal dominant disease), NOP10 or NHP2 (both autosomal recessive disease), which are part of the telomerase holoenzyme, have been identified in patients with dyskeratosis congenita. It may be that a defect in telomerase function due to Ruvbl2 mutation contributes to the T cell deficiency in Worker mice.
|Primers||Primers cannot be located by automatic search.|
Worker genotyping is performed by amplifying the region containing the mutation using PCR, followed by sequencing of the amplified region to detect the single nucleotide change.
Worker (F): 5’- TGTGACACGAAGCCTGTTTCCC -3’
Worker (R): 5’-CGGACACATGGTTCCAATGTTCCTC -3’
1) 95°C 2:00
2) 95°C 0:30
3) 56°C 0:30
4) 72°C 1:00
5) repeat steps (2-4) 29X
6) 72°C 7:00
7) 4°C ∞
Primers for sequencing
Worker_seq(F): 5’- ATTAGTGATTGATGGCCCAGAG -3’
Worker_seq(R): 5’- CCAATGTTCCTCAAAGTTCCAG -3’
The following sequence of 420 nucleotides (from Genbank genomic region NC_000073.5 for linear genomic sequence of Ruvbl2, sense strand) is amplified:
2887 tgtg acacgaagcc tgtttccctg ggccccgtgg tggggctgat cactgccatt
2941 agtgattgat ggcccagagg gtggtggtgg ctgctgttgt gttgcctgcc tgtgcagtgg
3001 ggggctcctg gtgggcagca ggaccttgag ggagcagatg aaactgtgac aactgggaac
3061 cttcttacac gtcatcgtcc tcacctgcag gcagccacca ccaaagtccc tgagatccga
3121 gatgtgacaa gaatcgagcg aatcggtgag tgagcagggt caggaccaag ggagacacca
3181 ctgcttagtg cccagacaga cagagaagga tgcaatgggg ccttagtccc aggctatgct
3241 gccatacgcc tagcatgcct ccacggggtt tctggaactt tgaggaacat tggaaccatg
Primer binding sites are underlined; sequencing primer binding sites are highlighted in gray; the mutated T is indicated in red.
1. Arnold, C. N., Pirie, E., Dosenovic, P., McInerney, G. M., Xia, Y., Wang, N., Li, X., Siggs, O. M., Karlsson Hedestam, G. B., and Beutler, B. (2012) A Forward Genetic Screen Reveals Roles for Nfkbid, Zeb1, and Ruvbl2 in Humoral Immunity. Proc. Natl. Acad. Sci. U. S. A.. .
2. Erzberger, J. P., and Berger, J. M. (2006) Evolutionary Relationships and Structural Mechanisms of AAA+ Proteins. Annu. Rev. Biophys. Biomol. Struct.. 35, 93-114.
3. Hishida, T., Han, Y. W., Fujimoto, S., Iwasaki, H., and Shinagawa, H. (2004) Direct Evidence that a Conserved Arginine in RuvB AAA+ ATPase Acts as an Allosteric Effector for the ATPase Activity of the Adjacent Subunit in a Hexamer. Proc. Natl. Acad. Sci. U. S. A.. 101, 9573-9577.
4. Ogura, T., Whiteheart, S. W., and Wilkinson, A. J. (2004) Conserved Arginine Residues Implicated in ATP Hydrolysis, Nucleotide-Sensing, and Inter-Subunit Interactions in AAA and AAA+ ATPases. J. Struct. Biol.. 146, 106-112.
5. Kanemaki, M., Makino, Y., Yoshida, T., Kishimoto, T., Koga, A., Yamamoto, K., Yamamoto, M., Moncollin, V., Egly, J. M., Muramatsu, M., and Tamura, T. (1997) Molecular Cloning of a Rat 49-kDa TBP-Interacting Protein (TIP49) that is Highly Homologous to the Bacterial RuvB. Biochem. Biophys. Res. Commun.. 235, 64-68.
6. Makino, Y., Kanemaki, M., Kurokawa, Y., Koji, T., and Tamura, T. (1999) A Rat RuvB-Like Protein, TIP49a, is a Germ Cell-Enriched Novel DNA Helicase. J. Biol. Chem.. 274, 15329-15335.
7. Kurokawa, Y., Kanemaki, M., Makino, Y., and Tamura, T. A. (1999) A Notable Example of an Evolutionary Conserved Gene: Studies on a Putative DNA Helicase TIP49. DNA Seq.. 10, 37-42.
8. Qiu, X. B., Lin, Y. L., Thome, K. C., Pian, P., Schlegel, B. P., Weremowicz, S., Parvin, J. D., and Dutta, A. (1998) An Eukaryotic RuvB-Like Protein (RUVBL1) Essential for Growth. J. Biol. Chem.. 273, 27786-27793.
9. Kanemaki, M., Kurokawa, Y., Matsu-ura, T., Makino, Y., Masani, A., Okazaki, K., Morishita, T., and Tamura, T. A. (1999) TIP49b, a New RuvB-Like DNA Helicase, is Included in a Complex Together with another RuvB-Like DNA Helicase, TIP49a. J. Biol. Chem.. 274, 22437-22444.
10. Eggleston, A. K., Mitchell, A. H., and West, S. C. (1997) In Vitro Reconstitution of the Late Steps of Genetic Recombination in E. Coli. Cell. 89, 607-617.
11. Tsaneva, I. R., Muller, B., and West, S. C. (1992) ATP-Dependent Branch Migration of Holliday Junctions Promoted by the RuvA and RuvB Proteins of E. Coli. Cell. 69, 1171-1180.
12. Matias, P. M., Gorynia, S., Donner, P., and Carrondo, M. A. (2006) Crystal Structure of the Human AAA+ Protein RuvBL1. J. Biol. Chem.. 281, 38918-38929.
13. Ikura, T., Ogryzko, V. V., Grigoriev, M., Groisman, R., Wang, J., Horikoshi, M., Scully, R., Qin, J., and Nakatani, Y. (2000) Involvement of the TIP60 Histone Acetylase Complex in DNA Repair and Apoptosis. Cell. 102, 463-473.
14. Torreira, E., Jha, S., Lopez-Blanco, J. R., Arias-Palomo, E., Chacon, P., Canas, C., Ayora, S., Dutta, A., and Llorca, O. (2008) Architecture of the pontin/reptin Complex, Essential in the Assembly of several Macromolecular Complexes. Structure. 16, 1511-1520.
15. Gribun, A., Cheung, K. L., Huen, J., Ortega, J., and Houry, W. A. (2008) Yeast Rvb1 and Rvb2 are ATP-Dependent DNA Helicases that Form a Heterohexameric Complex. J. Mol. Biol.. 376, 1320-1333.
16. Puri, T., Wendler, P., Sigala, B., Saibil, H., and Tsaneva, I. R. (2007) Dodecameric Structure and ATPase Activity of the Human TIP48/TIP49 Complex. J. Mol. Biol.. 366, 179-192.
17. Cheung, K. L., Huen, J., Houry, W. A., and Ortega, J. (2010) Comparison of the Multiple Oligomeric Structures Observed for the Rvb1 and Rvb2 Proteins. Biochem. Cell Biol.. 88, 77-88.
18. Cheung, K. L., Huen, J., Kakihara, Y., Houry, W. A., and Ortega, J. (2010) Alternative Oligomeric States of the Yeast Rvb1/Rvb2 Complex Induced by Histidine Tags. J. Mol. Biol.. 404, 478-492.
19. Niewiarowski, A., Bradley, A. S., Gor, J., McKay, A. R., Perkins, S. J., and Tsaneva, I. R. (2010) Oligomeric Assembly and Interactions within the Human RuvB-Like RuvBL1 and RuvBL2 Complexes. Biochem. J.. 429, 113-125.
20. Gorynia, S., Bandeiras, T. M., Pinho, F. G., McVey, C. E., Vonrhein, C., Round, A., Svergun, D. I., Donner, P., Matias, P. M., and Carrondo, M. A. (2011) Structural and Functional Insights into a Dodecameric Molecular Machine - the RuvBL1/RuvBL2 Complex. J. Struct. Biol.. 176, 279-291.
21. Parfait, B., Giovangrandi, Y., Asheuer, M., Laurendeau, I., Olivi, M., Vodovar, N., Vidaud, D., Vidaud, M., and Bieche, I. (2000) Human TIP49b/RUVBL2 Gene: Genomic Structure, Expression Pattern, Physical Link to the Human CGB/LHB Gene Cluster on Chromosome 19q13.3. Ann. Genet.. 43, 69-74.
22. Newman, D. R., Kuhn, J. F., Shanab, G. M., and Maxwell, E. S. (2000) Box C/D snoRNA-Associated Proteins: Two Pairs of Evolutionarily Ancient Proteins and Possible Links to Replication and Transcription. RNA. 6, 861-879.
23. King, T. H., Decatur, W. A., Bertrand, E., Maxwell, E. S., and Fournier, M. J. (2001) A Well-Connected and Conserved Nucleoplasmic Helicase is Required for Production of Box C/D and H/ACA snoRNAs and Localization of snoRNP Proteins. Mol. Cell. Biol.. 21, 7731-7746.
24. Jonsson, Z. O., Dhar, S. K., Narlikar, G. J., Auty, R., Wagle, N., Pellman, D., Pratt, R. E., Kingston, R., and Dutta, A. (2001) Rvb1p and Rvb2p are Essential Components of a Chromatin Remodeling Complex that Regulates Transcription of Over 5% of Yeast Genes. J. Biol. Chem.. 276, 16279-16288.
25. Shen, X., Ranallo, R., Choi, E., and Wu, C. (2003) Involvement of Actin-Related Proteins in ATP-Dependent Chromatin Remodeling. Mol. Cell. 12, 147-155.
26. Harata, M., Oma, Y., Mizuno, S., Jiang, Y. W., Stillman, D. J., and Wintersberger, U. (1999) The Nuclear Actin-Related Protein of Saccharomyces Cerevisiae, Act3p/Arp4, Interacts with Core Histones. Mol. Biol. Cell. 10, 2595-2605.
27. Downs, J. A., Allard, S., Jobin-Robitaille, O., Javaheri, A., Auger, A., Bouchard, N., Kron, S. J., Jackson, S. P., and Cote, J. (2004) Binding of Chromatin-Modifying Activities to Phosphorylated Histone H2A at DNA Damage Sites. Mol. Cell. 16, 979-990.
28. Shen, X., Mizuguchi, G., Hamiche, A., and Wu, C. (2000) A Chromatin Remodelling Complex Involved in Transcription and DNA Processing. Nature. 406, 541-544.
29. Ebbert, R., Birkmann, A., and Schuller, H. J. (1999) The Product of the SNF2/SWI2 Paralogue INO80 of Saccharomyces Cerevisiae Required for Efficient Expression of various Yeast Structural Genes is Part of a High-Molecular-Weight Protein Complex. Mol. Microbiol.. 32, 741-751.
30. Jin, J., Cai, Y., Yao, T., Gottschalk, A. J., Florens, L., Swanson, S. K., Gutierrez, J. L., Coleman, M. K., Workman, J. L., Mushegian, A., Washburn, M. P., Conaway, R. C., and Conaway, J. W. (2005) A Mammalian Chromatin Remodeling Complex with Similarities to the Yeast INO80 Complex. J. Biol. Chem.. 280, 41207-41212.
31. Jonsson, Z. O., Jha, S., Wohlschlegel, J. A., and Dutta, A. (2004) Rvb1p/Rvb2p Recruit Arp5p and Assemble a Functional Ino80 Chromatin Remodeling Complex. Mol. Cell. 16, 465-477.
32. Kobor, M. S., Venkatasubrahmanyam, S., Meneghini, M. D., Gin, J. W., Jennings, J. L., Link, A. J., Madhani, H. D., and Rine, J. (2004) A Protein Complex Containing the Conserved Swi2/Snf2-Related ATPase Swr1p Deposits Histone Variant H2A.Z into Euchromatin. PLoS Biol.. 2, E131.
33. Krogan, N. J., Keogh, M. C., Datta, N., Sawa, C., Ryan, O. W., Ding, H., Haw, R. A., Pootoolal, J., Tong, A., Canadien, V., Richards, D. P., Wu, X., Emili, A., Hughes, T. R., Buratowski, S., and Greenblatt, J. F. (2003) A Snf2 Family ATPase Complex Required for Recruitment of the Histone H2A Variant Htz1. Mol. Cell. 12, 1565-1576.
34. Mizuguchi, G., Shen, X., Landry, J., Wu, W. H., Sen, S., and Wu, C. (2004) ATP-Driven Exchange of Histone H2AZ Variant Catalyzed by SWR1 Chromatin Remodeling Complex. Science. 303, 343-348.
35. Cai, Y., Jin, J., Gottschalk, A. J., Yao, T., Conaway, J. W., and Conaway, R. C. (2006) Purification and Assay of the Human INO80 and SRCAP Chromatin Remodeling Complexes. Methods. 40, 312-317.
36. van Attikum, H., Fritsch, O., and Gasser, S. M. (2007) Distinct Roles for SWR1 and INO80 Chromatin Remodeling Complexes at Chromosomal Double-Strand Breaks. EMBO J.. 26, 4113-4125.
37. Tsukuda, T., Fleming, A. B., Nickoloff, J. A., and Osley, M. A. (2005) Chromatin Remodelling at a DNA Double-Strand Break Site in Saccharomyces Cerevisiae. Nature. 438, 379-383.
38. Cai, Y., Jin, J., Yao, T., Gottschalk, A. J., Swanson, S. K., Wu, S., Shi, Y., Washburn, M. P., Florens, L., Conaway, R. C., and Conaway, J. W. (2007) YY1 Functions with INO80 to Activate Transcription. Nat. Struct. Mol. Biol.. 14, 872-874.
39. Meneghini, M. D., Wu, M., and Madhani, H. D. (2003) Conserved Histone Variant H2A.Z Protects Euchromatin from the Ectopic Spread of Silent Heterochromatin. Cell. 112, 725-736.
40. Raisner, R. M., and Madhani, H. D. (2006) Patterning Chromatin: Form and Function for H2A.Z Variant Nucleosomes. Curr. Opin. Genet. Dev.. 16, 119-124.
41. Swaminathan, J., Baxter, E. M., and Corces, V. G. (2005) The Role of Histone H2Av Variant Replacement and Histone H4 Acetylation in the Establishment of Drosophila Heterochromatin. Genes Dev.. 19, 65-76.
42. Guillemette, B., and Gaudreau, L. (2006) Reuniting the Contrasting Functions of H2A.Z. Biochem. Cell Biol.. 84, 528-535.
43. van Attikum, H., Fritsch, O., Hohn, B., and Gasser, S. M. (2004) Recruitment of the INO80 Complex by H2A Phosphorylation Links ATP-Dependent Chromatin Remodeling with DNA Double-Strand Break Repair. Cell. 119, 777-788.
44. Morrison, A. J., Highland, J., Krogan, N. J., Arbel-Eden, A., Greenblatt, J. F., Haber, J. E., and Shen, X. (2004) INO80 and Gamma-H2AX Interaction Links ATP-Dependent Chromatin Remodeling to DNA Damage Repair. Cell. 119, 767-775.
45. Tsukuda, T., Lo, Y. C., Krishna, S., Sterk, R., Osley, M. A., and Nickoloff, J. A. (2009) INO80-Dependent Chromatin Remodeling Regulates Early and Late Stages of Mitotic Homologous Recombination. DNA Repair (Amst). 8, 360-369.
46. Kalocsay, M., Hiller, N. J., and Jentsch, S. (2009) Chromosome-Wide Rad51 Spreading and SUMO-H2A.Z-Dependent Chromosome Fixation in Response to a Persistent DNA Double-Strand Break. Mol. Cell. 33, 335-343.
47. Morrison, A. J., Kim, J. A., Person, M. D., Highland, J., Xiao, J., Wehr, T. S., Hensley, S., Bao, Y., Shen, J., Collins, S. R., Weissman, J. S., Delrow, J., Krogan, N. J., Haber, J. E., and Shen, X. (2007) Mec1/Tel1 Phosphorylation of the INO80 Chromatin Remodeling Complex Influences DNA Damage Checkpoint Responses. Cell. 130, 499-511.
48. Vincent, J. A., Kwong, T. J., and Tsukiyama, T. (2008) ATP-Dependent Chromatin Remodeling Shapes the DNA Replication Landscape. Nat. Struct. Mol. Biol.. 15, 477-484.
49. Shimada, K., Oma, Y., Schleker, T., Kugou, K., Ohta, K., Harata, M., and Gasser, S. M. (2008) Ino80 Chromatin Remodeling Complex Promotes Recovery of Stalled Replication Forks. Curr. Biol.. 18, 566-575.
50. Papamichos-Chronakis, M., and Peterson, C. L. (2008) The Ino80 Chromatin-Remodeling Enzyme Regulates Replisome Function and Stability. Nat. Struct. Mol. Biol.. 15, 338-345.
51. Hur, S. K., Park, E. J., Han, J. E., Kim, Y. A., Kim, J. D., Kang, D., and Kwon, J. (2010) Roles of Human INO80 Chromatin Remodeling Enzyme in DNA Replication and Chromosome Segregation Suppress Genome Instability. Cell Mol. Life Sci.. 67, 2283-2296.
52. Sun, Y., Jiang, X., and Price, B. D. (2010) Tip60: Connecting Chromatin to DNA Damage Signaling. Cell. Cycle. 9, 930-936.
53. Doyon, Y., Selleck, W., Lane, W. S., Tan, S., and Cote, J. (2004) Structural and Functional Conservation of the NuA4 Histone Acetyltransferase Complex from Yeast to Humans. Mol. Cell. Biol.. 24, 1884-1896.
54. Jha, S., Shibata, E., and Dutta, A. (2008) Human Rvb1/Tip49 is Required for the Histone Acetyltransferase Activity of Tip60/NuA4 and for the Downregulation of Phosphorylation on H2AX After DNA Damage. Mol. Cell. Biol.. 28, 2690-2700.
55. Frank, S. R., Parisi, T., Taubert, S., Fernandez, P., Fuchs, M., Chan, H. M., Livingston, D. M., and Amati, B. (2003) MYC Recruits the TIP60 Histone Acetyltransferase Complex to Chromatin. EMBO Rep.. 4, 575-580.
56. Taubert, S., Gorrini, C., Frank, S. R., Parisi, T., Fuchs, M., Chan, H. M., Livingston, D. M., and Amati, B. (2004) E2F-Dependent Histone Acetylation and Recruitment of the Tip60 Acetyltransferase Complex to Chromatin in Late G1. Mol. Cell. Biol.. 24, 4546-4556.
57. DeRan, M., Pulvino, M., Greene, E., Su, C., and Zhao, J. (2008) Transcriptional Activation of Histone Genes Requires NPAT-Dependent Recruitment of TRRAP-Tip60 Complex to Histone Promoters during the G1/S Phase Transition. Mol. Cell. Biol.. 28, 435-447.
58. Murr, R., Loizou, J. I., Yang, Y. G., Cuenin, C., Li, H., Wang, Z. Q., and Herceg, Z. (2006) Histone Acetylation by Trrap-Tip60 Modulates Loading of Repair Proteins and Repair of DNA Double-Strand Breaks. Nat. Cell Biol.. 8, 91-99.
59. Kusch, T., Florens, L., Macdonald, W. H., Swanson, S. K., Glaser, R. L., Yates, J. R.,3rd, Abmayr, S. M., Washburn, M. P., and Workman, J. L. (2004) Acetylation by Tip60 is Required for Selective Histone Variant Exchange at DNA Lesions. Science. 306, 2084-2087.
60. Bird, A. W., Yu, D. Y., Pray-Grant, M. G., Qiu, Q., Harmon, K. E., Megee, P. C., Grant, P. A., Smith, M. M., and Christman, M. F. (2002) Acetylation of Histone H4 by Esa1 is Required for DNA Double-Strand Break Repair. Nature. 419, 411-415.
61. Sun, Y., Xu, Y., Roy, K., and Price, B. D. (2007) DNA Damage-Induced Acetylation of Lysine 3016 of ATM Activates ATM Kinase Activity. Mol. Cell. Biol.. 27, 8502-8509.
62. Sun, Y., Jiang, X., Chen, S., Fernandes, N., and Price, B. D. (2005) A Role for the Tip60 Histone Acetyltransferase in the Acetylation and Activation of ATM. Proc. Natl. Acad. Sci. U. S. A.. 102, 13182-13187.
63. Watkins, N. J., Dickmanns, A., and Luhrmann, R. (2002) Conserved Stem II of the Box C/D Motif is Essential for Nucleolar Localization and is Required, Along with the 15.5K Protein, for the Hierarchical Assembly of the Box C/D snoRNP. Mol. Cell. Biol.. 22, 8342-8352.
64. Watkins, N. J., Lemm, I., Ingelfinger, D., Schneider, C., Hossbach, M., Urlaub, H., and Luhrmann, R. (2004) Assembly and Maturation of the U3 snoRNP in the Nucleoplasm in a Large Dynamic Multiprotein Complex. Mol. Cell. 16, 789-798.
65. McKeegan, K. S., Debieux, C. M., Boulon, S., Bertrand, E., and Watkins, N. J. (2007) A Dynamic Scaffold of Pre-snoRNP Factors Facilitates Human Box C/D snoRNP Assembly. Mol. Cell. Biol.. 27, 6782-6793.
66. McKeegan, K. S., Debieux, C. M., and Watkins, N. J. (2009) Evidence that the AAA+ Proteins TIP48 and TIP49 Bridge Interactions between 15.5K and the Related NOP56 and NOP58 Proteins during Box C/D snoRNP Biogenesis. Mol. Cell. Biol.. 29, 4971-4981.
67. Zhao, R., Davey, M., Hsu, Y. C., Kaplanek, P., Tong, A., Parsons, A. B., Krogan, N., Cagney, G., Mai, D., Greenblatt, J., Boone, C., Emili, A., and Houry, W. A. (2005) Navigating the Chaperone Network: An Integrative Map of Physical and Genetic Interactions Mediated by the hsp90 Chaperone. Cell. 120, 715-727.
68. Zhao, R., Kakihara, Y., Gribun, A., Huen, J., Yang, G., Khanna, M., Costanzo, M., Brost, R. L., Boone, C., Hughes, T. R., Yip, C. M., and Houry, W. A. (2008) Molecular Chaperone Hsp90 Stabilizes Pih1/Nop17 to Maintain R2TP Complex Activity that Regulates snoRNA Accumulation. J. Cell Biol.. 180, 563-578.
69. Cloutier, P., Al-Khoury, R., Lavallee-Adam, M., Faubert, D., Jiang, H., Poitras, C., Bouchard, A., Forget, D., Blanchette, M., and Coulombe, B. (2009) High-Resolution Mapping of the Protein Interaction Network for the Human Transcription Machinery and Affinity Purification of RNA Polymerase II-Associated Complexes. Methods. 48, 381-386.
70. Horejsi, Z., Takai, H., Adelman, C. A., Collis, S. J., Flynn, H., Maslen, S., Skehel, J. M., de Lange, T., and Boulton, S. J. (2010) CK2 Phospho-Dependent Binding of R2TP Complex to TEL2 is Essential for mTOR and SMG1 Stability. Mol. Cell. 39, 839-850.
71. Boulon, S., Marmier-Gourrier, N., Pradet-Balade, B., Wurth, L., Verheggen, C., Jady, B. E., Rothe, B., Pescia, C., Robert, M. C., Kiss, T., Bardoni, B., Krol, A., Branlant, C., Allmang, C., Bertrand, E., and Charpentier, B. (2008) The Hsp90 Chaperone Controls the Biogenesis of L7Ae RNPs through Conserved Machinery. J. Cell Biol.. 180, 579-595.
72. Gonzales, F. A., Zanchin, N. I., Luz, J. S., and Oliveira, C. C. (2005) Characterization of Saccharomyces Cerevisiae Nop17p, a Novel Nop58p-Interacting Protein that is Involved in Pre-rRNA Processing. J. Mol. Biol.. 346, 437-455.
73. Wood, M. A., McMahon, S. B., and Cole, M. D. (2000) An ATPase/helicase Complex is an Essential Cofactor for Oncogenic Transformation by c-Myc. Mol. Cell. 5, 321-330.
74. Izumi, N., Yamashita, A., Iwamatsu, A., Kurata, R., Nakamura, H., Saari, B., Hirano, H., Anderson, P., and Ohno, S. (2010) AAA+ Proteins RUVBL1 and RUVBL2 Coordinate PIKK Activity and Function in Nonsense-Mediated mRNA Decay. Sci. Signal.. 3, ra27.
75. Venteicher, A. S., Meng, Z., Mason, P. J., Veenstra, T. D., and Artandi, S. E. (2008) Identification of ATPases Pontin and Reptin as Telomerase Components Essential for Holoenzyme Assembly. Cell. 132, 945-957.
76. Bosma, G. C., Custer, R. P., and Bosma, M. J. (1983) A Severe Combined Immunodeficiency Mutation in the Mouse. Nature. 301, 527-530.
77. Nijnik, A., Dawson, S., Crockford, T. L., Woodbine, L., Visetnoi, S., Bennett, S., Jones, M., Turner, G. D., Jeggo, P. A., Goodnow, C. C., and Cornall, R. J. (2009) Impaired Lymphocyte Development and Antibody Class Switching and Increased Malignancy in a Murine Model of DNA Ligase IV Syndrome. J. Clin. Invest.. 119, 1696-1705.
78. Rooney, S., Sekiguchi, J., Zhu, C., Cheng, H. L., Manis, J., Whitlow, S., DeVido, J., Foy, D., Chaudhuri, J., Lombard, D., and Alt, F. W. (2002) Leaky Scid Phenotype Associated with Defective V(D)J Coding End Processing in Artemis-Deficient Mice. Mol. Cell. 10, 1379-1390.
|Science Writers||Eva Marie Y. Moresco, Anne Murray|
|Illustrators||Diantha La Vine|
|Authors||Carrie N. Arnold, Elaine Pirie, and Bruce Beutler|