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Viruses 2014, 6(3), 968-985; doi:10.3390/v6030968
Published: 26 February 2014
Abstract: Human cytomegalovirus (HCMV) is a ubiquitous pathogen capable of causing life threatening consequences in neonates and immune-compromised individuals. HCMV inflicts site-specific double strand breaks (DSBs) in the cellular genome. DNA damage infliction raises the corollary question of virus modulation of DNA repair. We recently reported HDR was stimulated in wt human foreskin fibroblasts (HFFs) during fully permissive infection or expression of the HCMV protein IE1-72 (IE72). These studies have been extended into semi-permissive T98G glioblastoma cells. T98Gs encode a mutant p53, which may contribute to their high baseline rate of HDR. We fully expected HCMV infection to increase HDR in T98Gs, similar to its effects in HFFs. Surprisingly in T98Gs HCMV infection, or sole expression of IE72, decreased HDR by two-fold. Transient expression of wt p53 in T98Gs also reduced HDR by two-fold. Dual transient expression of wt p53 and IE72 restored high baseline HDR levels. GST pulldown experiments revealed that both IE72 and wt p53 bound the important HDR protein, Rad51. We conclude that the expression of certain HCMV proteins can modulate HDR in an infected cell, dependent upon p53 status. We propose a model of the protein interactions explaining this behavior.
Human cytomegalovirus (HCMV) is a member of the β-herpesvirus family and is endemic in the human population. HCMV can cause congenital birth defects, primarily of neurological origin [1,2,3]. It also causes severe systemic disease following reactivation in immunosuppressed individuals . The virus’ role in oncomodulation of cancers has also recently been the subject of intensive investigation (for review see [5,6]).
One of the direct effects of HCMV infection in human foreskin fibroblasts (HFFs), is the induction of two site-specific breaks at chromosome 1q42 and 1q23.3 in the host cellular DNA [7,8]. The physiological significance of HCMV-induced specific breaks or whether they can be repaired is unknown. However, the proximity of the 1q23.3 breakpoint to two hearing impairment (HI) loci, DFNA49 and DFNA7, and in the vicinity of the myelin protein zero (MPZ) gene , prompts speculation on this break’s correlation with the hearing loss observed in congenitally infected infants.
Mammalian cells are exposed to both intrinsic (i.e., reactive oxygen species) and extrinsic (i.e., genotoxic chemicals) agents capable of inflicting cellular DNA damage. DNA damage triggers a cascade of complex protein signaling pathways. This combination of pathways constitutes the DNA damage response (DDR). Depending on the type and extent of DNA damage different repair pathways are activated. In the case of double-stranded breaks (DSBs), two repair pathways are principally activated (as reviewed in [10,11]). One is the error free homology-directed repair (HDR) pathway, which commonly involves strand invasion of a sister chromatid. The other pathway utilizes the more error-prone non-homologous end-joining (NHEJ) or single-strand annealing mechanisms.
We recently reported interactions between HCMV and HDR in permissive HFFs . HCMV infection caused a two-fold increase in HDR of an I-SceI induced site-specific DNA DSB, from a baseline level of 4% to a stimulated level of 8%. Expression of the HCMV IE72 protein on its own produced comparable results. Here the same DSB repair assay has found that HCMV regulates HDR in the semi-permissive T98G cells in a surprising and counterintuitive manner, hinging on the p53 status of these cells. A model to explain the interaction of HCMV IE72 with p53 and the HDR machinery is proposed.
2.1. Introduction of the pDRGFP Substrate into T98G Cells to Assess HDR
Our earlier study assessed whether HCMV infection affected HDR of an integrated substrate at I-SceI-induced DSBs in fully permissive HFFs. This work found that HDR, as measured by an increase in GFP+ cells, was stimulated in HFFs during HCMV infection and, further, that expression of the HCMV protein IE72 on its own also stimulated HDR . The assay utilized a non-functional GFP reporter substrate susceptible to DSBs upon introduction of I-SceI [13,14] (see Figure 1A for diagram of the substrate). If the DSB was successfully repaired by HDR, functional GFP was reconstituted. HDR was scored by microscopic analysis for cellular GFP+. These fibroblast experiments have now been extended into the semi-permissive cell line T98G. Three different stable clones of T98Gs with an integrated pDRGFP substrate were generated. The results obtained using all clones were consistent, therefore here we report only representative studies carried out in Clone 10.
Clone 10 was synchronized in G0 and then infected with an Adenovirus (Ad) expressing the I-SceI endonuclease (NGUS24i), or an Ad control virus (dL70-3) [15,16] at various MOIs (5, 10, 25, 50, 100, and 200) or were mock-infected. Cells were analyzed for efficiency of I-SceI endonuclease production after NGUS24i infection. The I-SceI endonuclease in this virus is tagged with hemagglutinin (HA), permitting detection of protein expression using an anti-HA Ab by IF. 100% of the cells infected with NGUS24i displayed HA-positivity and no staining was observed in mock-infected cells (Figure 1B) or dL70-3-infected cells (data not shown).
NGUS24i infection produced GFP+ cells. This indicated I-SceI-induced site-specific DNA breaks had been successfully repaired by HDR. In our hands NGUS24i infection effects were greatest using an MOI of 200 and continuous incubation for 72 h prior to harvest. Clone 10 was also examined for spontaneous HDR events. Figure 1B displays representative experiments depicting the absence of any GFP+ cells in mock-infected Clone 10. These results demonstrated that the Ad-based enzyme delivery system in conjunction with the integrated pDRGFP substrate worked as well in the T98G cells as had been previously observed in the HFFs .
2.2. HDR at I-SceI Induced DSBs Was Downregulated in HCMV-Infected T98G Cells
Previously we showed that in a semi-permissive infection of T98G cells, although all cells take up virus, only a modest percentage (~30%–40%) of cells express IE72 antigen (Ag) in contrast to 100% Ag+ cells in a fully permissive infection . Clone 10 was Go synchronized, released from synchronization and then mock-infected or HCMV-infected at an MOI of 10 for 48 h. These cells were subsequently superinfected with NGUS24i or dL70-3 and harvested at 72 h post Ad infection. Cells were stained for the expression of HCMV IE72 by IF to monitor initiation and progression of HCMV infection. Approximately 30% of cells were IE72+ at 120 h post infection (hpi), which agreed with previous experiments . Cells were also scored for GFP+. Representative IF images for these infections are shown in Figure 2A.
T98Gs displayed a very high baseline rate of HDR after DSB induction with I-SceI. Ad NGUS24i infection resulted in ~16% GFP+ cells (as compared to 4% in HFFs) . No GFP+ cells were observed in either dL70-3-infected or mock-infected cells. An average of ~7% GFP+ cells were detected in HCMV-infected cells subsequently superinfected with NGUS24i to induce DSBs, an ~2 fold decrease (Figure 2B). Although not quite reaching a degree of statistical significance, this decrease was consistently reproducible (fold changes of 2.7 and 1.9 in two experiments). Downregulation of HDR due to HCMV infection was not associated with changes in steady state levels of I-SceI expression. Immunoblot analysis found no decrease in I-SceI expression in HCMV-infected T98Gs compared to mock-infected T98Gs (Figure 2C). Actually, somewhat the reverse was found with slightly higher levels of I-SceI observed in lysates derived from an equivalent number of virus-infected cells. Thus lower expression of the I-SceI enzyme was not the cause of the somewhat paradoxical decrease in HDR.
2.3. Transient Expression of IE72 Alone Was Sufficient to Downregulate HDR in T98Gs
A number of studies have suggested that IE72 plays a vital role in fine tuning the host cell, including activating early gene expression needed for viral replication ( and as reviewed in ). We had previously shown that expression of IE72 alone was sufficient to enhance HDR in HFFs . Having found that full HCMV infection reduced HDR in T98Gs, we repeated the IE72 expression assays in these cells. Parallel experiments to those above were performed in Clone 10 nucleofected with vector-alone (pSG5) or an IE72-expressing construct (pSGIE72). These cells were then Ad infected. Cells were subsequently scored for IE72 and GFP positivity. Approximately 90% cells were IE72+ (data not shown).
No GFP+ cells were observed in vector alone (pSG5), pSG5 + dL70-3-infected (control Ad), IE72 alone or IE72 + dL70-3-infected cells. In close agreement with the previous results an average of ~16 % GFP+ cells were detected in cells nucleofected with pSG5 and NGUS24i-infected (I-SceI expressing Ad). In cells nucleofected with the IE72 construct and NGUS24i-infected, an average of 9% GFP+ cells were scored, a 1.8 fold decrease (Figure 3A). This decrease was approximately equivalent to the reduction in GFP+ of HCMV-infected cells. Again, although this decrease was not statistically significant, it was consistently reproducible (fold changes of 1.9 and 1.5 in two experiments). Therefore, as was seen in HFFs, transient expression of IE72 alone largely recapitulated the HCMV-infection results, however, with the same perplexing downregulation of HDR in T98Gs.
2.4. Expression of wt p53 in T98Gs Caused the Same Decrease in HDR as IE72
T98Gs have a mutagenic profile and harbor a mutation in p53 at R273H, in the DNA binding domain . It is widely accepted that wt p53 suppresses HDR (as reviewed in ). Was the mutation in p53 responsible for the elevated levels of HDR (~16%, Figure 2B) in uninfected T98Gs compared to HFFs (~4%, )? If so, introduction of wt p53 would be expected to decrease HDR levels in uninfected T98G cells and, similarly, p53 DNA binding domain mutants would not be expected to alter HDR levels. Experiments parallel to those discussed for IE72 were performed in Clone 10. It should be noted that although all the constructs used in this study were GFP-tagged, the wt p53 and the mutant p53 genes were expressed from the weak wt p53 promoter and, as we have previously observed , no detectable GFP expression above background was observed in control populations of these cells (data not shown). Clone 10 was nucleofected with vector-alone (pCDNA3-T7) or constructs  expressing wt p53, a non-acetylatable p53 mutant (K382R), p53 DNA binding domain mutants (R273H, R175H, R248W, G154V), or a p53 N-terminal multi-site phosphorylation mutant and subsequently Ad-infected. Cells were scored for GFP+ (Figure 3B).
Immediately evident was that introduction of even low levels of wt p53 into T98Gs resulted in accelerated cell death, with very few cells surviving until 72 h post Ad infection. The infection protocol was modified to overcome this technical problem. Ad infection MOIs were reduced from 200 to 5. An MOI of 5 still delivered I-SceI enzyme to the entire population, as detected by HA Ab staining (data not shown), however the lower MOI reduced baseline DSB-induced HDR events to a more modest, but still prevalent, ~11%. More importantly, the reduced MOI allowed sufficiently high cell survival for a long enough duration to obtain meaningful population counts. Eight hours post‑nucleofection, cells were Ad infected and GFP+ was scored at 40 h post Ad infection. Following this modified protocol, control experiments using any of the constructs followed by infection with the dL70-3 control virus showed no GFP+ cells (data not shown). Nucleofection with no DNA, or introduction of vector alone (pCDNA3) followed by I-SceI-expressing NGUS24i-infection produced an average ~11% GFP+ cells (Figure 3B). Cells nucleofected with wt p53 or the p53 K382R mutant produced an average of ~6% GFP+, an ~2 fold decrease. This decrease was consistently reproducible and highly statistically significant for both constructs (p value < 0.0001 and 0.0004, respectively). The introduction of the p53 DNA binding domain mutants (R273H, R175H, R248W, G154V), or the p53 N-terminal multi-site phosphorylation mutant yielded no change in the percent of GFP+ from the vector alone. Thus, introduction of wt p53 into the T98G cells suppressed the high level HDR allowed by the endogenous mutant p53 .
2.5. Co-Expression of IE72 and wt p53 Negated Their Individual Effects on HDR
Surprisingly, in the T98G microenvironment, expression of either IE72 or wt p53 reduced HDR, therefore we tested co-introduction of both proteins. Using the modified protocol described above, once again control experiments using dL70-3 virus produced no GFP+ cells (data not shown). We observed that nucleofection with no DNA, or introduction of backbone vector (pCDNA3) followed by I-SceI-expressing NGUS24i produced an average ~9% GFP+ cells. Introduction of either IE72 or wt p53 alone reduced GFP+ to ~5%, an ~2 fold decrease as expected, both of which were statistically significant (p = 0.01 and p = 0.0014, respectively). Much to our surprise, dual introduction of IE72 and wt p53 produced an average of 13.6% GFP+ cells, an ~1.4 fold increase from the baseline rate of ~9%, an increase that was only marginally statistically significant (p = 0.043) (fold changes of 1.3, 1.7, 1.5 in three experiments) (Figure 3C). This suggested that in T98G cells interaction between wt p53 and IE72 negated their individual effects on the HDR machinery.
2.6. In Vitro Binding Assays Found Both wt p53 and IE72 Bound Rad51
T98G cells harbor a mutant p53 (R273H mutation) . The mutation abolishes specific DNA binding. The p53 transient expression experiments established that an intact DNA binding domain and phosphorylatable N-terminus were required to decrease HDR in these cells. Previous studies have determined that recombination is controlled, at least in part, by p53 binding to the strand invasion protein Rad51, which modulates Rad51’s function (as reviewed in ). An intact DNA binding domain in the p53 protein is required for this interaction [23,24,25]. Further, T98G cells mount a DSB response  and express high levels of the DSB repair proteins, including Rad51 [20,26]. Previous work had established that p53 could bind both Rad51 and IE72 , and that interaction between p53 and IE72 could negate p53’s normal DNA binding ability through its core region . This information suggested that the effects noted in the above transient expression and co-expression experiments might be the result of IE72 binding either wt p53 or Rad51. In vitro mixing experiments of radiolabeled Rad51 and pGEX72, GST wt p53 or pGEX-KG (control GST alone) were performed. As can be seen in Figure 4, both p53 and IE72 were capable of binding Rad51, although IE72 appeared to be slightly less avid for the protein. While not excluding other possible explanations, this binding, in combination with the results from the expression experiments, have prompted us to propose a protein interaction model capable of explaining the observed behaviors (see Figure 5 below). This model may have significant bearing on questions entirely unrelated to HCMV-infection in the semi‑permissive cell type T98G.
3. Experimental Section
3.1. Cells and Virus Growth
T98G glioblastoma cells and clones expressing pDRGFP were propagated in Earle’s minimal essential media (MEM) supplemented with 10% heat-inactivated fetal bovine serum (FBS), L‑glutamine (2 mM), penicillin (200 U/mL), streptomycin (200 mg/mL), and amphotericin B (1.5 mg/mL). Cells were grown in incubators maintained at 37 °C and 5% CO2. The Towne strain of HCMV was obtained from the ATCC (# VR 977), propagated under standard procedures and used at a multiplicity of infection (MOI) of 10 in all experiments. The recombinant Ad strains dL70-3, used as a control virus, and NGUS24i, encoding the I-SceI enzyme, (both kind gifts of Frank Graham and Philip Ng, McMaster University, Hamilton, ON, Canada [15,16]) were grown and titrated in replication-permissive human 293A cells. The MOI of Ad viruses used was established separately depending on experimental procedure (see above for particular details).
Lipofectamine reagent (Invitrogen/Life Technologies, Grand Island, NY, USA) was used according to manufacturer’s instructions to introduce pDRGFP [13,14] into T98Gs. Following transfection, cells were grown in non-selective medium for 48 h. Subsequently, puromycin (1 mg/mL) was added to the media to select for integrated pDRGFP. Cloning rings were used to isolate puromycin-resistant colonies. Colonies were separated and subjected to another cycle of puromycin selection prior to freezing and storage in liquid nitrogen. All colonies were tested to ensure the absence of GFP+ without DSB induction. Three stable clones of T98GpDRGFP were tested and produced comparable results in the assays described above. T98GpDRGFP clone 10 (Clone 10) was used for all experiments reported here.
Nucleofection of T98Gs was optimized using a protocol provided by Amaxa Biosystems (program O-016). Each nucleofection used ~5 × 105 cells. IE72 transient expression studies used either 6 µg of control vector pSG5 (Stratagene/Agilent Technologies, Santa Clara, CA, USA) or 6 µg of pSGIE72 . p53 transient expression experiments used the following constructs in the listed quantities: 6 µg of vector pCDNA3-T7 alone (with the CMV promoter removed, as a control) or 6 µg of p53 derivative vectors containing (1) a wt p53 promoter-wt p53-green fluorescent protein (GFP) cassette (wtp53pCDNA3-T7) or (2) an equivalent vector cassette containing one of the following p53 mutations: K382R, R273H, R175H, R248W, G154V or an N-terminal multi-site phosphorylation mutant . All of these have been previously described . After nucleofection, cells were immediately transferred to plates containing coverslips and pre-warmed medium.
3.4. Molecular Cloning
The pCDNA3-T7 vector was modified by insertion into its polylinker of a BamHI-NotI fragment containing DsRed2 (from pDsRed2-N1vector; Clontech Laboratories, Mountain View, CA, USA) to produce pCDNA3-DsRed. The wt p53 promoter-wt p53 coding sequence was cleaved from pCLNCX-p53pro-p53GFP  at the KpnI and AgeI sites. Finally, this fragment was inserted upstream of DsRed2 in the polylinker of pCDNA3-DsRed. This ultimately produced the pCDNA3-p53pro-p53DsRed construct. Dual transient expression studies with wt p53 and IE72 used 3 µg each of pCDNA3-p53pro-p53DsRed and pSGIE72. Alternatively, one of these constructs (3 µg) was transfected along with the corresponding control backbone of the other construct (3 µg).
3.5. DSB Repair Assay
The DSB repair assay was carried out as described previously . The results reported were carried out in mock- or HCMV-infected Clone 10.
3.6. Virus Infection
Clone 10 was synchronized in Go by serum starvation for 3 d. Cells were then washed with PBS, trypsinized and re-plated at a density of 5 or 10 × 105 cells/60-mm dish containing glass coverslips. After allowing 2 h for attachment, the cells were mock- or HCMV-infected. Twenty-four hours later the virus or mock inoculums were removed (unless otherwise noted). After an additional 24 h, cells were washed once with PBS and subsequently superinfected for 30 minutes in pre-warmed media. Super-infection was with control Ad dL70-3 or with I-SceI-expressing Ad NGUS24i . Cells were then re-fed with complete media. Cells were fixed and permeabilized 72 h later unless otherwise noted. Coverslips were scored for GFP+ cells and IE72+ cells.
3.7. Antibodies (Ab)
Primary mouse monoclonal antibodies (mAbs) used were: anti-pan actin (IgG1) (Neomarkers/Thermo Scientific, Fremont, CA, USA); anti‑hemagglutinin (HA)(12CA5) (IgG2b)(Abcam, Cambridge, MA, USA); anti-IE1 (IgG2a) (a kind gift from Bill Britt, University of Alabama, Birmingham, AL, USA); and anti-IE1 and -IE2 (Ch16.0; IgG1) (Virusys Corporation, Taneytown, MD, USA). Secondary Abs used were as follows: for immunoblot detection, horseradish peroxidase (HRP)-linked sheep anti-mouse (GE Healthcare Life Sciences, Pittsburgh, PA, USA), and for IF analysis, tetramethyl rhodamine isothiocyanate (TRITC)-conjugated anti-mouse IgG1, IgG2a and IgG2b (Jackson ImmunoResearch Laboratories, West Grove, PA, USA).
3.8. Immunofluorescence (IF)
Cells were seeded into dishes containing glass coverslips. Coverslips were collected and processed at indicated times pi, as described previously . 300–500 cells per coverslip were counted and scored for GFP+ and either HA+ or IE72+ cells in each experiment. All experimental results represent the average of at least two independent experiments. Error bars represent +/− one standard deviation (SD). Statistical analysis was performed using unpaired, two-tailed student t-tests.
3.10. GST Binding Studies
Overnight bacterial cultures (100 mL in LB + 100 μg/mL ampicillin) containing the GST fusion plasmids pGEX-human p53 (1-393) (Addgene plasmid #24860; ), pGEX72  or pGEX-KG  were diluted 1:10 (to a final volume of 1 L LB/amp) and incubated an additional 1 h at 37 °C with shaking. Cultures were chilled to room temperature (RT), then 1 mL 0.5M IPTG was added. After an additional incubation at RT for 2 h, bacteria were pelleted at 5000 rpm for 10 min and cells were resuspended in 50 mL NETN + protease inhibitors (PIs) (20 mM Tris pH 8, 100 mM NaCl, 1 mM EDTA, 0.5% NP40, 2 mg/mL aprotinin, 2 mg/mL leupeptin, 100 mM DTT). This suspension was then frozen at −80 °C in 5 mL aliquots for future use.
Assays were performed using one of the 5 mL aliquots thawed on ice. Fifty μL of a 10 mg/mL lysozyme solution was added and the cell suspension was incubated on ice for 30 min. The suspension was sonically disrupted to lyse the cells. Debris was pelleted at 10,000 rpm for 5 min and the supernatant transferred to a new tube. Sixty μL of a 50% glutathione agarose bead slurry (vol/vol in NETN) was added and rocked at 4 °C for 1 h. Beads were then washed in 500 μL NETN + PIs three times prior to final re-suspension in 500 μL NETN + PIs. Fifty μL of this bead suspension (25 μL bead equivalents) were incubated with 20 μL Laemmli reducing sample buffer (2% SDS, 10% glycerol, 100 mM DTT, 60 mM Tris pH 6.8, Bromophenol blue dye, aprotinin and leupeptin (2 μg/mL each)), and then boiled for 5 min. The resulting supernatant was loaded onto a 12% SDS-PAGE gel. The gel was stained with Coomassie dye to visualize the GST fusion proteins and to determine equivalent protein amounts for use in the following binding reactions. Roughly equivalent amounts of protein, as estimated from the Coomassie staining, were used in the reactions (approximately 30 μL beads of pGEX72 and pGEX-p53 and 7.5 μL of pGEX-KG were used in the reactions shown in Figure 4).
Pet24d-Rad51  was in vitro translated using the Promega quick-coupled TNT reaction kit per manufacturer’s instructions. In each binding assay, five μL of translated Rad51 (or just TNT reaction mixture) was incubated while rocking for 1 h at 4 °C with the GST fusion proteins in a 500 μL reaction of NETN + PIs. After incubation, 40 μL of a 50% Protein A Sepharose slurry (vol/vol in NETN) was added to each tube (to increase the bead volume). Ten percent of the total volume (54 μL) was removed to serve as the input fraction (no washes of these beads followed). The beads in the remaining sample were pelleted and then washed four times with 500 μL of buffer (the first two washes in NETN, the last two in RIPA (150 mM NaCl, 1% Nonidet P-40, 0.5% deoxycholate, 0.1% SDS, 50 mM Tris (pH 8), 5 mM EDTA). After the final spin, 15 μL of urea sample buffer was added to the beads and the samples were boiled for 5 min. The supernatants were run on a 12% SDS‑PAGE gel. Gels were dried and exposed to Kodak X-omat film.
A cell’s ability to repair insult to its DNA is a process that is essential to its survival. The concept that virus infection may alter this capability has begun to be investigated. In theory a virus might benefit from manipulation of the repair processes, while simultaneously (and likely corollary) degrading the integrity of a host’s genome. Existing studies have examined a variety of different repair pathways in the context of expression of a single viral protein and have assessed that protein’s capability to influence the repair of exogenously introduced damage in the cellular DNA [35,36,37,38,39,40,41,42,43,44,45,46]. The effects on repair during a complete infection have also been examined [12,47,48,49,50,51,52,53,54,55,56]. A handful of these studies have looked specifically at HDR [12,35,37,45,49]. The very large majority of these studies found viral protein expression (or full infection) decreased cellular repair capabilities.
Two cellular proteins, p53 and Rad51, are exceedingly important in the context of HDR. It is widely accepted that wt p53 regulates HDR, primarily through interactions with Rad51 (as reviewed in ). In vitro reactions have found p53 binds Rad51 and, by means of this interaction, inhibits strand exchange and branch migration of recombination intermediates . An intact core DNA binding domain of the p53 protein is required for direct binding between the p53 and Rad51 proteins (and inhibition of the latter’s activities) [23,24,25]. It has also been shown that following induction of damage wt p53 inhibits transactivation of the Rad51 promoter, thereby acting as a repressor of Rad51 transcription and protein expression . It has also been shown that a phosphorylatable N-terminus is important for regulation and binding of Rad51 . Many tumors (and cell lines derived from them) have so called “hotspot” mutations in p53, including the T98G cells used in this study . Reintroduction of wt p53 into these tumor cells reduced HDR via decreasing Rad51 activity .
Multiple viruses have been shown to interact with the Rad51 protein. Epstein-Barr Virus (EBV), a herpesvirus, and SV40 have both been found to require the presence of Rad51 within their viral replication centers. Knockdown of Rad51 in infected cells dramatically decreased viral replication [60,61]. The opposite was true for HIV; stimulation of Rad51 activity inhibited HIV replication, primarily due to an inhibitory effect of Rad51 on the virus’ Integrase enzyme .
The context of the T98G cellular environment is important for consideration of HDR in these cells. Under normal stress T98Gs can complete HDR and have normal levels of Rad51 . Baseline levels of HDR in T98G cells after insult are quite high, perhaps in part due to the large proportion of these rapidly dividing cells being in the S/G2 phases of the cell cycle, during which HDR is most common [25,59]. However, the higher rate of HDR may also be attributable to the presence of the mutation in the p53 DNA binding domain (R273H) within these cells , which prevents p53’s normal binding to, and regulation of, Rad51.
The model in Figure 5 is proposed to explain the dichotomy of results between the T98G results reported here and our earlier HFF study. In wt cells p53 normally inhibits Rad51 activity. In the model, the prediction is that the mutant p53-containing T98G cells, where p53 cannot bind Rad51 [23,24,25], would have high baseline recombination rates, as seen. The model further predicts that, introduction on their own (indicated by the arrow in the figure) of either wt p53 or IE72 (which we have shown can bind Rad51 in vitro) into these cells would decrease HDR by their binding to and inhibiting Rad51. Co-expression of both wt p53 and IE72 did not inhibit Rad51. We propose in these experiments wt p53 and IE72 bound to one another, inhibiting normal p53 activity . This seems a reasonable assumption, given previous reports that IE72 binds directly to p53 and inhibits core domain binding ability . If the introduced wt p53 and IE72 were interacting and p53’s normal activity was inhibited, Rad51 would again be free to cause the high recombination rates observed.
Also in our model, in wt cells p53 normally inhibits Rad51, establishing baseline HDR activity levels. HCMV-infection of wt fibroblast cells causes p53 to become tightly associated with the viral replication centers . We believe in an infected cell this viral manipulation of p53 prevents the normal binding of p53 and Rad51. The disruption of this normal condition in turn frees Rad51 to increase recombination in both the viral and cellular DNA. Experiments in wt cells found that expression of the single HCMV protein IE72 was sufficient to increase HDR levels . The proposed model attributes the increase in HDR in wt cells to IE72 binding to wt p53, thereby inhibiting the ability of wt p53 to bind and regulate Rad51.
The proposed model offers a mechanistic explanation for our previously reported results in wt HFFs . The focus of the earlier HFF study was the recognition of viral manipulation of a cellular repair mechanism to its own ends in the context of a fully permissive infection. The experiments performed in T98G cells were expected to corroborate that data. Fortuitously, the particular microenvironment of the mutant glioblastoma cells allowed elucidation of what we believe to be the protein interactions responsible.
The results of this study may have implications for the initiation of glioblastomas. It has been reported that in excess of 90% of glioblastomas contain HCMV genetic material [64,65]. A latently HCMV-infected neural progenitor/stem cell which reactivated could, and most likely would, express IE72. We have found that expression of IE72 in a wt cell was capable of increasing unscheduled recombination, a hallmark of genetic instability and perhaps the first step toward hyperproliferation and gliomagenesis. The common perception of HCMV as a relatively harmless pathogen belie not only its capacity to cause serious birth defects, inflict direct DNA damage and downregulate repair of the cellular genome, but perhaps its capability to initiate an often lethal and devastating cancer. We have experiments underway to determine if the protein interactions found in this study are capable of intitiating oncogenic effects in tissue culture experiments.
This work was supported by NIH grants # RO1-AI51463 and #P20 RR015587 (COBRE program) to EAF. The authors would like to thank John O’Dowd for critical reading of the manuscript.
Conflicts of Interest
The authors declare no conflict of interest.
References and Notes
- Boppana, S.B.; Fowler, K.B.; Britt, W.J.; Stagno, S.; Pass, R.F. Symptomatic congenital cytomegalovirus infection in infants born to mothers with preexisting immunity to cytomegalovirus. Pediatrics 1999, 104, 55–60, doi:10.1542/peds.104.1.55.
- Cinque, P.; Marenzi, R.; Ceresa, D. Cytomegalovirus infections of the nervous system. Intervirology 1997, 40, 85–97, doi:10.1159/000150536.
- Zanghellini, F.; Boppana, S.B.; Emery, V.C.; Griffiths, P.D.; Pass, R.F. Asymptomatic primary cytomegalovirus infection: Virologic and immunologic features. J. Infect. Dis. 1999, 180, 702–707, doi:10.1086/314939.
- Britt, W.; Alford, C. Cytomegalovirus. In Fields Virology; Lippincott-Raven Publishers: Philadelphia, PA, USA, 1996; pp. 2493–2523.
- Dziurzynski, K.; Wei, J.; Qiao, W.; Hatiboglu, M.A.; Kong, L.Y.; Wu, A.; Wang, Y.; Cahill, D.; Levine, N.; Prabhu, S.; et al. Glioma-associated cytomegalovirus mediates subversion of the monocyte lineage to a tumor propagating phenotype. Clin. Canc. Res. 2011, 17, 4642–4649, doi:10.1158/1078-0432.CCR-11-0414.
- Michaelis, M.; Baumgarten, P.; Mittelbronn, M.; Driever, P.H.; Doerr, H.W.; Cinatl, J., Jr. Oncomodulation by human cytomegalovirus: Novel clinical findings open new roads. Med. Microbiol. Immunol. 2011, 200, 1–5, doi:10.1007/s00430-010-0177-7.
- Fortunato, E.A.; Dell'Aquila, M.L.; Spector, D.H. Specific chromosome 1 breaks induced by human cytomegalovirus. Proc. Natl. Acad. Sci. USA 2000, 97, 853–858, doi:10.1073/pnas.97.2.853.
- Nystad, M.; Fagerheim, T.; Brox, V.; Fortunato, E.A.; Nilssen, O. Human cytomegalovirus (HCMV) and hearing impairment: Infection of fibroblast cells with HCMV induces chromosome breaks at 1q23.3, between loci DFNA7 and DFNA49—Both involved in dominantly inherited, sensorineural, hearing impairment. Mutat. Res. 2008, 637, 56–65, doi:10.1016/j.mrfmmm.2007.07.009.
- Toesca, A. Central and peripheral myelin in the rat cochlear and vestibular nerves. Neurosci. Lett. 1996, 221, 21–24, doi:10.1016/S0304-3940(96)13273-0.
- Chapman, J.R.; Taylor, M.R.; Boulton, S.J. Playing the end game: DNA double-strand break repair pathway choice. Mol. Cell 2012, 47, 497–510, doi:10.1016/j.molcel.2012.07.029.
- Rothkamm, K.; Kruger, I.; Thompson, L.H.; Lobrich, M. Pathways of DNA double-strand break repair during the mammalian cell cycle. Mol. Cell Biol. 2003, 23, 5706–5715, doi:10.1128/MCB.23.16.5706-5715.2003.
- Kulkarni, A.S.; Fortunato, E.A. Stimulation of homology-directed repair at I-SceI-induced DNA breaks during the permissive life cycle of human cytomegalovirus. J. Virol. 2011, 85, 6049–6054, doi:10.1128/JVI.02514-10.
- Pierce, A.J.; Johnson, R.D.; Thompson, L.H.; Jasin, M. Xrcc3 promotes homology-directed repair of DNA damage in mammalian cells. Genes Dev. 1999, 13, 2633–2638, doi:10.1101/gad.13.20.2633.
- Wiese, C.; Pierce, A.J.; Gauny, S.S.; Jasin, M.; Kronenberg, A. Gene conversion is strongly induced in human cells by double-strand breaks and is modulated by the expression of bcl-x(l). Canc. Res. 2002, 62, 1279–1283.
- Bett, A.J.; Haddara, W.; Prevec, L.; Graham, F.L. An efficient and flexible system for construction of adenovirus vectors with insertions or deletions in early regions 1 and 3. Proc. Natl. Acad. Sci. USA 1994, 91, 8802–8806, doi:10.1073/pnas.91.19.8802.
- Anglana, M.; Bacchetti, S. Construction of a recombinant adenovirus for efficient delivery of the I-SceI yeast endonuclease to human cells and its application in the in vivo cleavage of chromosomes to expose new potential telomeres. Nucleic Acids Res. 1999, 27, 4276–4281, doi:10.1093/nar/27.21.4276.
- Luo, M.H.; Fortunato, E.A. Long-term infection and shedding of human cytomegalovirus in T98G glioblastoma cells. J. Virol. 2007, 81, 10424–10436, doi:10.1128/JVI.00866-07.
- Greaves, R.F.; Mocarski, E.S. Defective growth correlates with reduced accumulation of a viral DNA replication protein after low-multiplicity infection by a human cytomegalovirus IE1 mutant. J. Virol. 1998, 72, 366–379.
- Castillo, J.P.; Kowalik, T.F. Human cytomegalovirus immediate early proteins and cell growth control. Gene 2002, 290, 19–34, doi:10.1016/S0378-1119(02)00566-8.
- Short, S.C.; Bourne, S.; Martindale, C.; Woodcock, M.; Jackson, S.P. DNA damage responses at low radiation doses. Rad. Res. 2005, 164, 292–302, doi:10.1667/RR3421.1.
- Bertrand, P.; Saintigny, Y.; Lopez, B.S. P53's double life: Transactivation-independent repression of homologous recombination. Trends Gen. 2004, 20, 235–243, doi:10.1016/j.tig.2004.04.003.
- Rosenke, K.; Samuel, M.A.; McDowell, E.T.; Toerne, M.A.; Fortunato, E.A. An intact sequence-specific DNA-binding domain is required for human cytomegalovirus-mediated sequestration of p53 and may promote in vivo binding to the viral genome during infection. Virology 2006, 348, 19–34, doi:10.1016/j.virol.2005.12.013.
- Arias-Lopez, C.; Lazaro-Trueba, I.; Kerr, P.; Lord, C.J.; Dexter, T.; Iravani, M.; Ashworth, A.; Silva, A. P53 modulates homologous recombination by transcriptional regulation of the Rad51 gene. EMBO Rep. 2006, 7, 219–224, doi:10.1038/sj.embor.7400587.
- Buchhop, S.; Gibson, M.K.; Wang, X.W.; Wagner, P.; Sturzbecher, H.W.; Harris, C.C. Interaction of p53 with the human Rad51 protein. Nucleic Acids Res. 1997, 25, 3868–3874, doi:10.1093/nar/25.19.3868.
- Rieckmann, T.; Kriegs, M.; Nitsch, L.; Hoffer, K.; Rohaly, G.; Kocher, S.; Petersen, C.; Dikomey, E.; Dornreiter, I.; Dahm-Daphi, J. P53 modulates homologous recombination at I-SceI-induced double-strand breaks through cell-cycle regulation. Oncogene 2013, 32, 968–975, doi:10.1038/onc.2012.123.
- Daboussi, F.; Dumay, A.; Delacote, F.; Lopez, B.S. DNA double-strand break repair signalling: The case of Rad51 post-translational regulation. Cell Signal. 2002, 14, 969–975, doi:10.1016/S0898-6568(02)00052-9.
- Hwang, E.S.; Zhang, Z.; Cai, H.; Huang, D.Y.; Huong, S.M.; Cha, C.Y.; Huang, E.S. Human cytomegalovirus IE1–72 protein interacts with p53 and inhibits p53-dependent transactivation by a mechanism different from that of IE2–86 protein. J. Virol. 2009, 83, 12388–12398, doi:10.1128/JVI.00304-09.
- Klucher, K.M.; Sommer, M.; Kadonaga, J.T.; Spector, D.H. In vivo and in vitro analysis of transcriptional activation mediated by the human cytomegalovirus major immediate-early proteins. Mol. Cell Biol. 1993, 13, 1238–1250.
- Ashcroft, M.; Kubbutat, M.H.; Vousden, K.H. Regulation of p53 function and stability by phosphorylation. Mol. Cell Biol. 1999, 19, 1751–1758.
- Casavant, N.C.; Luo, M.H.; Rosenke, K.; Winegardner, T.; Zurawska, A.; Fortunato, E.A. Potential role for p53 in the permissive life cycle of human cytomegalovirus. J. Virol. 2006, 80, 8390–8401, doi:10.1128/JVI.00505-06.
- Luo, M.H.; Rosenke, K.; Czornak, K.; Fortunato, E.A. Human cytomegalovirus disrupts both ataxia telangiectasia mutated protein (ATM)- and ATM-Rad3-related kinase-mediated DNA damage responses during lytic infection. J. Virol. 2007, 81, 1934–1950, doi:10.1128/JVI.01670-06.
- Ayed, A.; Mulder, F.A.; Yi, G.S.; Lu, Y.; Kay, L.E.; Arrowsmith, C.H. Latent and active p53 are identical in conformation. Nat. Struct. Biol. 2001, 8, 756–760, doi:10.1038/nsb0901-756.
- Guan, K.L.; Dixon, J.E. Eukaryotic proteins expressed in Escherichia coli: An improved thrombin cleavage and purification procedure of fusion proteins with glutathione s-transferase. Anal. Biochem. 1991, 192, 262–267, doi:10.1016/0003-2697(91)90534-Z.
- Snowden, T.; Shim, K.S.; Schmutte, C.; Acharya, S.; Fishel, R. hMSH4-hMSH5 adenosine nucleotide processing and interactions with homologous recombination machinery. J. Biol. Chem. 2008, 283, 145–154, doi:10.1074/jbc.M704060200.
- Baydoun, H.H.; Pancewicz, J.; Nicot, C. Human T-lymphotropic type 1 virus p30 inhibits homologous recombination and favors unfaithful DNA repair. Blood 2011, 117, 5897–5906, doi:10.1182/blood-2010-08-304600.
- Becker, S.A.; Lee, T.H.; Butel, J.S.; Slagle, B.L. Hepatitis B virus X protein interferes with cellular DNA repair. J. Virol. 1998, 72, 266–272.
- Chipitsyna, G.; Slonina, D.; Siddiqui, K.; Peruzzi, F.; Skorski, T.; Reiss, K.; Sawaya, B.E.; Khalili, K.; Amini, S. HIV-1 Tat increases cell survival in response to cisplatin by stimulating Rad51 gene expression. Oncogene 2004, 23, 2664–2671, doi:10.1038/sj.onc.1207417.
- Durkin, S.S.; Guo, X.; Fryrear, K.A.; Mihaylova, V.T.; Gupta, S.K.; Belgnaoui, S.M.; Haoudi, A.; Kupfer, G.M.; Semmes, O.J. HTLV-1 Tax oncoprotein subverts the cellular DNA damage response via binding to DNA-dependent protein kinase. J. Biol. Chem. 2008, 283, 36311–36320, doi:10.1074/jbc.M804931200.
- Groisman, I.J.; Koshy, R.; Henkler, F.; Groopman, J.D.; Alaoui-Jamali, M.A. Downregulation of DNA excision repair by the hepatitis B virus-X protein occurs in p53-proficient and p53-deficient cells. Carcinogenesis 1999, 20, 479–483, doi:10.1093/carcin/20.3.479.
- Gruhne, B.; Sompallae, R.; Masucci, M.G. Three Epstein-Barr virus latency proteins independently promote genomic instability by inducing DNA damage, inhibiting DNA repair and inactivating cell cycle checkpoints. Oncogene 2009, 28, 3997–4008, doi:10.1038/onc.2009.258.
- Jia, L.; Wang, X.W.; Harris, C.C. Hepatitis B virus X protein inhibits nucleotide excision repair. Int. J. Canc. 1999, 80, 875–879, doi:10.1002/(SICI)1097-0215(19990315)80:6<875::AID-IJC13>3.0.CO;2-Z.
- Liang, X.; Pickering, M.T.; Cho, N.H.; Chang, H.; Volkert, M.R.; Kowalik, T.F.; Jung, J.U. Deregulation of DNA damage signal transduction by herpesvirus latency-associated M2. J. Virol. 2006, 80, 5862–5874, doi:10.1128/JVI.02732-05.
- Prost, S.; Ford, J.M.; Taylor, C.; Doig, J.; Harrison, D.J. Hepatitis B X protein inhibits p53-dependent DNA repair in primary mouse hepatocytes. J. Biol. Chem. 1998, 273, 33327–33332.
- Sun, Y.; Huang, Y.C.; Xu, Q.Z.; Wang, H.P.; Bai, B.; Sui, J.L.; Zhou, P.K. HIV-1 Tat depresses DNA-PK(cs) expression and DNA repair, and sensitizes cells to ionizing radiation. Int. J. Radiat. Oncol. Biol. Phys. 2006, 65, 842–850, doi:10.1016/j.ijrobp.2006.02.040.
- Trojanek, J.; Croul, S.; Ho, T.; Wang, J.Y.; Darbinyan, A.; Nowicki, M.; Valle, L.D.; Skorski, T.; Khalili, K.; Reiss, K. T-antigen of the human polyomavirus JC attenuates faithful DNA repair by forcing nuclear interaction between IRS-1 and Rad51. J. Cell. Physiol. 2006, 206, 35–46, doi:10.1002/jcp.20425.
- Mathonnet, G.; Lachance, S.; Alaoui-Jamali, M.; Drobetsky, E.A. Expression of hepatitis B virus X oncoprotein inhibits transcription-coupled nucleotide excision repair in human cells. Mutat. Res. 2004, 554, 305–318, doi:10.1016/j.mrfmmm.2004.05.010.
- Mohni, K.N.; Mastrocola, A.S.; Bai, P.; Weller, S.K.; Heinen, C.D. DNA mismatch repair proteins are required for efficient herpes simplex virus 1 replication. J. Virol. 2011, 85, 12241–12253, doi:10.1128/JVI.05487-11.
- O'Dowd, J.M.; Zavala, A.G.; Brown, C.J.; Mori, T.; Fortunato, E.A. HCMV-infected cells maintain efficient nucleotide excision repair of the viral genome while abrogating repair of the host genome. PLoS Pathog. 2012, 8, e1003038, doi:10.1371/journal.ppat.1003038.
- Schumacher, A.J.; Mohni, K.N.; Kan, Y.; Hendrickson, E.A.; Stark, J.M.; Weller, S.K. The HSV-1 exonuclease, UL12, stimulates recombination by a single strand annealing mechanis. PLoS Pathog. 2012, 8, e1002862, doi:10.1371/journal.ppat.1002862.
- Deng, C.Z.; AbuBakar, S.; Fons, M.P.; Boldogh, I.; Hokanson, J.; Au, W.W.; Albrecht, T. Cytomegalovirus-enhanced induction of chromosome aberrations in human peripheral blood lymphocytes treated with potent genotoxic agents. Environ. Mol. Mutagen. 1992, 19, 304–310.
- Duong, F.H.; Christen, V.; Lin, S.; Heim, M.H. Hepatitis C virus-induced up-regulation of protein phosphatase 2a inhibits histone modification and DNA damage repair. Hepatology 2010, 51, 741–751.
- Lilley, C.E.; Chaurushiya, M.S.; Boutell, C.; Landry, S.; Suh, J.; Panier, S.; Everett, R.D.; Stewart, G.S.; Durocher, D.; Weitzman, M.D. A viral E3 ligase targets RNF8 and RNF168 to control histone ubiquitination and DNA damage responses. EMBO J. 2010, 29, 943–955, doi:10.1038/emboj.2009.400.
- Pal, S.; Polyak, S.J.; Bano, N.; Qiu, W.C.; Carithers, R.L.; Shuhart, M.; Gretch, D.R.; Das, A. Hepatitis C virus induces oxidative stress, DNA damage and modulates the DNA repair enzyme NEIL1. J. Gastroenterol. Hepatol. 2010, 25, 627–634, doi:10.1111/j.1440-1746.2009.06128.x.
- Philpott, S.M.; Buehring, G.C. Defective DNA repair in cells with human T-cell leukemia/bovine leukemia viruses: Role of Tax gene. J. Natl. Canc. Inst. 1999, 91, 933–942, doi:10.1093/jnci/91.11.933.
- Ranneberg-Nilsen, T.; Bjoras, M.; Luna, L.; Slettebakk, R.; Dale, H.A.; Seeberg, E.; Rollag, H. Human cytomegalovirus infection modulates DNA base excision repair in fibroblast cells. Virology 2006, 348, 389–397, doi:10.1016/j.virol.2006.01.001.
- Bowman, K.K.; Sicard, D.M.; Ford, J.M.; Hanawalt, P.C. Reduced global genomic repair of ultraviolet light-induced cyclobutane pyrimidine dimers in simian virus 40-transformed human cells. Mol. Carcinog. 2000, 29, 17–24, doi:10.1002/1098-2744(200009)29:1<17::AID-MC3>3.0.CO;2-E.
- Yoon, D.; Wang, Y.; Stapleford, K.; Wiesmuller, L.; Chen, J. P53 inhibits strand exchange and replication fork regression promoted by human Rad51. J. Mol. Biol. 2004, 336, 639–654, doi:10.1016/j.jmb.2003.12.050.
- Restle, A.; Janz, C.; Wiesmuller, L. Differences in the association of p53 phosphorylated on serine 15 and key enzymes of homologous recombination. Oncogene 2005, 24, 4380–4387, doi:10.1038/sj.onc.1208639.
- Mekeel, K.L.; Tang, W.; Kachnic, L.A.; Luo, C.M.; DeFrank, J.S.; Powell, S.N. Inactivation of p53 results in high rates of homologous recombination. Oncogene 1997, 14, 1847–1857.
- Boichuk, S.; Hu, L.; Hein, J.; Gjoerup, O.V. Multiple DNA damage signaling and repair pathways deregulated by simian virus 40 large T antigen. J. Virol. 2010, 84, 8007–8020, doi:10.1128/JVI.00334-10.
- Kudoh, A.; Iwahori, S.; Sato, Y.; Nakayama, S.; Isomura, H.; Murata, T.; Tsurumi, T. Homologous recombinational repair factors are recruited and loaded onto the viral DNA genome in Epstein-Barr virus replication compartments. J. Virol. 2009, 83, 6641–6651, doi:10.1128/JVI.00049-09.
- Cosnefroy, O.; Tocco, A.; Lesbats, P.; Thierry, S.; Calmels, C.; Wiktorowicz, T.; Reigadas, S.; Kwon, Y.; De Cian, A.; Desfarges, S.; et al. Stimulation of the human Rad51 nucleofilament restricts HIV-1 integration in vitro and in infected cells. J. Virol. 2012, 86, 513–526, doi:10.1128/JVI.05425-11.
- Fortunato, E.A.; Spector, D.H. P53 and RPA are sequestered in viral replication centers in the nuclei of cells infected with human cytomegalovirus. J. Virol. 1998, 72, 2033–2039.
- Dziurzynski, K.; Chang, S.M.; Heimberger, A.B.; Kalejta, R.F.; McGregor Dallas, S.R.; Smit, M.; Soroceanu, L.; Cobbs, C.S. HCMV Glioma Symposium. Consensus on the role of human cytomegalovirus in glioblastoma. Neuro Oncol. 2012, 14, 246–255, doi:10.1093/neuonc/nor227.
- Ranganathan, P.; Clark, P.A.; Kuo, J.S.; Salamat, M.S.; Kalejta, R.F. Significant association of multiple human cytomegalovirus genomic loci with glioblastoma multiforme samples. J. Virol. 2012, 86, 854–864, doi:10.1128/JVI.06097-11.
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