DNA interstrand crosslinks (ICLs) are toxic lesions that block the progression of replication and transcription. CtIP is a conserved DNA repair protein that facilitates DNA end resection in the double-strand break (DSB) repair pathway. Here we show that CtIP plays a critical role during initiation of ICL processing in replicating human cells that is distinct from its role in DSB repair. CtIP depletion sensitizes human cells to ICL inducing agents and significantly impairs the accumulation of DNA damage response proteins RPA, ATR, FANCD2, γH2AX, and phosphorylated ATM at sites of laser generated ICLs. In contrast, the appearance of γH2AX and phosphorylated ATM at sites of laser generated double strand breaks (DSBs) is CtIP-independent. We present a model in which CtIP functions early in ICL repair in a BRCA1– and FANCM–dependent manner prior to generation of DSB repair intermediates.
One of the most lethal forms of DNA damage is the interstrand crosslink (ICL). An ICL is a chemical bridge between two nucleotides on complementary strands of DNA. An unrepaired ICL is toxic because it poses an unsurpassable block to DNA replication and transcription. Certain forms of cancer treatment exploit the toxicity of ICL generating agents to target rapidly dividing cells. Sensitivity to crosslinking agents is a defining characteristic of Fanconi Anemia (FA), a hereditary syndrome characterized by an increased risk in cancer development and hematopoietic abnormalities frequently resulting in bone marrow failure. The mechanism underlying ICL repair is important to human health; however, the sequence of molecular events governing ICL repair is poorly understood. Here we describe how the repair protein CtIP functions to initiate ICL repair in replicating cells in a manner distinct from its previously described role in other forms of DNA repair.
Citation: Duquette ML, Zhu Q, Taylor ER, Tsay AJ, Shi LZ, Berns MW, et al. (2012) CtIP Is Required to Initiate Replication-Dependent Interstrand Crosslink Repair. PLoS Genet 8(11): e1003050. doi:10.1371/journal.pgen.1003050
Editor: James M. Ford, Stanford University School of Medicine, United States of America
Received: December 5, 2011; Accepted: September 12, 2012; Published: November 8, 2012
Copyright: © 2012 Duquette et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This work was funded by National Institutes of Health (NIH) grant #R01CA095114 to CHM and by NIH/NCI Ruth L. Kirschstein National Research Service Award F32 CA128399 to MLD. QZ, LZS, and MWB were supported by a U.S. Air force grant #AFOSR FA9550-08-1-0384 to MWB and the Beckman Laser Institute Foundation, Irvine, California. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Cellular DNA can be chemically modified and damaged when exposed to environmental agents, metabolic byproducts, or chemotherapeutic agents. The most toxic of these lesions is the interstrand crosslink (ICL), a covalent bridge formed between complementary strands of DNA. If not repaired, ICLs prevent DNA strand separation resulting in a block to replication and transcription. ICL generating agents are commonly used in the treatment of cancer. Sensitivity to crosslinking agents is a defining characteristic of Fanconi Anemia (FA), a rare hereditary syndrome characterized by an increased risk in cancer development and hematopoetic abnormalities frequently resulting in bone marrow failure . Elucidation of the cellular pathways that repair ICLs is highly relevant to understanding carcinogenesis, development of novel therapies to treat FA patients, and to the development of better targeted chemotherapeutic drugs.
Sensitivity assays suggest that eukaryotic cells have evolved multiple complex systems to repair ICLs that involve the intersection of several different repair pathways (reviewed in , ). However, the specific mechanism by which ICLs are detected and repair is initiatedremains unknown. A major ICL repair pathway in higher eukaryotes functions during S-phase and is thought to be replication dependent –. ICLs can also be repaired in a replication independent manner –. Current models of replication mediated ICL repair, suggest that repair is initiated when a fork stalls due to encountering an ICL , . FANCM/FAAP24 then binds to the ICL stalled fork –. Next, single stranded DNA (ssDNA) is generated and bound by RPA , ,  and the DNA damage response kinase ATR/ATRIP localizes to the damaged chromatin through binding to RPA . Localization of ATR/ATRIP to damaged DNA is essential for activation of the S-phase checkpoint and ICL repair , . The ability of ICLs to activate the checkpoint is dependent on the FA core complex (FANCA/B/C/E/F/G/M) , but not FANCI-FAND2 . The generation of ssDNA at stalled replication forks is thought to be critical for ATR activation. However, the factors required to generate ssDNA under circumstances in which the ICL poses a structural barrier to helicase uncoupling from the DNA polymerase at the replication fork are not known . It has been shown ssDNA arises at an ICL stalled fork in Xenopus extracts due to resection of the lagging strand . In addition this ssDNA is competent for Rad51 loading prior to generation of a DSB ICL repair intermediate .
The FANCI-FANCD2 complex is phosphorylated by activated ATR in response to ICL stalled replication forks , , . This phosphorylation facilitates FANCI-FANCD2 monoubiquitination by the FA core complex , . Monoubiquitination is essential for localization of the FANCI-FANCD2 complex to damaged chromatin where it directs downstream repair steps , –. The FANCI-FANCD2 complex is required for the initial ICL incision step in replication competent Xenopus extracts .
Several candidate nucleases have been identified that may function to excise the ICL. These nucleases include XPF/ERCC1, MUS81/EME1, their regulator SLX4 (also known as the Fanconi Anemia gene FANCP) –, SNM1A ,  and SNM1B . Whether they act redundantly or in concert is not clear, however they are all characterized by showing higher sensitivity to crosslinking agents compared to other forms of damage. MUS81/EME1 and XPF/ERCC1 have been proposed to function both early , and late in the ICL repair process –, , . The nuclease FAN1 also confers resistance to ICL inducing agents and has been shown to interact physically with the monoubiquitinated form of the FANCD2 nuclease –. Although a large number of nucleases are implicated in ICL repair, it remains unclear at which specific step these proteins exert their functions.
Following ICL incision, translesion synthesis by an error prone polymerase repairs the strand opposite the incised ICL , –. Excision of the ICL and polymerase extension up to the excised region results in the generation of double stranded ends resembling a double strand break (DSB). The DSB is repaired by homologous recombination as evidenced by the extreme sensitivity of homologous recombination impaired cell lines to ICL inducing agents –.
We hypothesized that CtIP might play an important and unique role in replication dependent ICL repair for the following reasons. First, studies of the CtIP homologs in A. thaliana (AtGR1) and S. cerevisiae (SAE2) have revealed a conserved role for CtIP in ICL repair due to their ability to confer resistance to the ICL inducing agent mitomycin C (MMC) , . Second, CtIP expression is enhanced in S through G2 phase ,  when ICL repair primarily occurs. Third, CtIP plays a conserved role in coordinating the recognition and resection of double strand breaks with the MRE11-RAD50-NBS1 (MRN) complex – and may act to facilitate the generation of ssDNA ends following ICL incision.
To investigate the mechanism of ICL repair in live mammalian cells we developed a system that takes advantage of the chemical and physical characteristics of the cross-linking agent, 8-methoxy psoralen (8-MOP). 8-MOP intercalates into DNA and forms DNA ICLs upon exposure to long wavelength UVA light (365 nm) . In this system we used laser directed 2-photon activation of 8-MOP via infrared light (730 nm) to generate ICLs in individual human S-phase nuclei. This approach restricts damage to precisely defined subnuclear volumes allowing one to monitor the spatiotemporal dynamics of DNA repair factors after ICL induction. This system was used to determine what role CtIP plays in ICL repair. We show that CtIP plays an important and unexpectedly early role in ICL repair in S phase human cells. In addition to the known role of CtIP and MRE11 in DSB end resection , , , the data presented here demonstrates that CtIP plays an additional role in ICL repair prior to generation of DSB repair intermediates. The data show that CtIP acts prior to RPA loading and localization of ATR and FANCD2 to ICL containing DNA. CtIP is required for the accumulation of known DSB repair factors phospho-histone H2AX (γH2AX), and ATM autophosphorylated on serine-1981 (ATM-pS1981) at ICLs, but not at DSBs. The data support a model in which CtIP is recruited to ICLs in a FANCM dependent manner and is required to initiate ICL processing of stalled forks prior to ICL incision.
CtIP depletion sensitizes cells to ICL inducing agents
To determine if CtIP plays a role in ICL repair, we assayed CtIP depleted human cells for sensitivity to the ICL inducing agents MMC or 8-MOP plus whole cell UVA irradiation (365 nm). The products of activated 8-MOP on DNA are predominantly ICLs, but monoadducts are also formed , . The psoralen angelicin, which is structurally related to 8-MOPs, forms monoadducts upon UVA exposure and was used to control for cellular sensitivity to DNA monoadducts . CtIP was depleted from Human Embryonic Kidney Cells (HEK293) by transient transfection of two previously described independent small interfering RNAs (siRNAs) . Luciferase siRNA was used as a nontargeting control. CtIP RNA levels were monitored by RT-qPCR and were found to be reduced on average by 70%. Sensitivity to ICL and monoadduct inducing compounds was determined by assessing the fraction of surviving cells after 8 days. As shown in Figure 1A, CtIP depleted cells were sensitive to the ICL inducing agents 8-MOP+UVA and to MMC. CtIP depleted cells were not sensitive to angelicin plus UVA. CtIP depleted cells were only slightly sensitive to IR induced DSBs (Figure S1). This sensitivity profile is similar to that reported for A. thaliana AtGR1/AtCom1 mutated cells , and suggests that CtIP plays an important and conserved role in ICL repair.
(A) Left, Survival of HEK293 cells transfected with control or CtIP siRNAs and exposed to 8-MOP+UVA or angelicin+UVA. CtIP_1 and CtIP_2 are two independent siRNAs. Cells were treated with indicated drug 48 hours post transfection and survival was assessed 8 days post irradiation. Fraction surviving cells is calculated in respect to untreated cells. Right, Survival of control or CtIP depleted cells treated 8 days following exposure to indicated concentration of MMC. Bars indicate standard deviation between 3 independent experiments. (B) γH2AX staining of fixed HeLa cells 2 hours post microirradiation with 730 nm laser light. S-phase synchronized cells were treated with indicated drugs prior to laser microirradiation. Black line on phase images indicates region of nucleus targeted by the laser. Thymidine arrested cells were microirradiated in the presence of 8-MOP. (C) Quantification of cells scored as having bright γH2AX staining along laser tracks. For details on cell analysis see Experimental Procedures. Bars indicate standard deviation between 3 independent experiments.
Generation of ICLs by 2-photon activation of 8-MOP
To define the role of CtIP in ICL repair, we established a system that enables the examination of the spatial and temporal recruitment and retention of repair proteins at region specific ICLs. An analogous approach has been used to generate study ICL repair using a UV laser plus light activated psoralen , . Our approach uses a near infrared femtosecond laser to produce 730 nm light which activates 8-methoxypsoralen (8-MOP) by two-photon activation (effective wavelength of 365 nm at the focal point). This enabled us to define precisely a subnuclear volume in which DNA damage was created while avoiding damage outside the focal points . This method allowed specific activation of 8-MOP with doses of light that caused no detectable damage in psoralen free control cells (Figure 1B).
To define the optimal laser power, we first identified the lowest laser power that gave a robust γH2AX signal in cells treated with 8-MOP, and no observable γH2AX by laser alone (Figure 1B). Cells were subject to thymidine block and release to enrich for replicating cells . One hour after thymidine release the indicated drug was added, and cells were microirradiated with 730 nm light using a femtosecond laser. Following microirradiation, cells were maintained in culture for 2 hours allowing time for replication forks to encounter the damage prior to fixation (Figure S2). Angelicin was used as a control for the amount of γH2AX at the laser tracks that resulted from the generation and/or processing of monoadducts. To verify that the γH2AX along laser tracks was replication dependent a control experiment was performed in which cells were held in thymidine during drug treatment and laser microirradiation. γH2AX staining signal along microirradiated tracks was quantified in individual cells using Image J (See Materials and Methods). The proportion of cells with positive γH2AX staining along microirradiated tracks are summarized in Figure 1C. The number of cells scored positive for γH2AX signal along laser tracks was highly increased in S-phase cells microirradiated in the presence of 8-MOP (83%) relative to microirradiated drug free cells (0%) (n = 29 and 25 cells respectively). Blocking replication in 8-MOP microirradiated cells reduced the number of γH2AX positive cells almost to background levels (4.5%) (n = 21). Angelicin treated microirradiated cells did not yield bright γH2AX signal (0%) (n = 25) (Figure 1B, 1C), however we do not exclude the possibility that adduct formation by angelicin may be less efficient than that of 8-MOP. Thus we conclude that the γH2AX signal detected in 8-MOP microirradiated cells is primarily due to the replication dependent processing of ICLs.
Previously published reports have shown that CtIP plays a role in G1/S progression in mouse fibroblasts (MEFs, NIH 3T3) , . We wanted to examine whether CtIP depletion affected cell cycle and S-phase progression in HeLa which could have an effect on the efficiency of ICL repair. Cell cycle analysis was performed on CtIP depleted and control HeLa cells. No significant difference in cell cycle distribution was observed between control cells and 2 independent CtIP siRNAs in 3 independent experiments (Figure 2A, 2B). Figure 2C shows that both CtIP siRNAs effectively depleted CtIP in the samples analyzed for cell cycle distribution. Quantification of the nucleotide analog bromodeoxyuridine (BrdU) incorporation in individual siRNA transfected cells was determined to compare the number of S phase cells and the relative rates of replication associated nucleotide incorporation under the same conditions used in laser experiments. ICL detection and initiation of repair in S phase occurs primarily when a replication fork encounters and stalls at an ICL. Therefore it was important to verify that fork progression, as determined by BrdU incorporation, is not affected in CtIP depleted cells relative to control cells. As judged by quantification of pixel intensities in individual cells there was no significant difference in replication rate between control and CtIP depleted cells Figure 2D. In addition, under the conditions used for laser irradiation experiments >95% of the cells were in S phase. The lack of an effect on cell cycle distribution or BrdU incorporation in CtIP depleted HeLa cells suggests that the decrease in γH2AX generation at ICLs in CtIP depleted cells is due to a defect in ICL processing as opposed to a cell cycle progression defect.
(A) Cell cycle profiles of control and siCtIP transfected HeLa cells 48 hours after transfection. Labels mark the cell populations in the G1 (left peak), S (saddle), and G2 (right peak) phases of the cell cycle based on their DNA content. (B) Summary of cell cycle distributions in control and siRNA transfected HeLa cells. Percentages shown are averages of the results of 3 experiments ± the standard deviations. There was no significant difference between the cell cycle distributions of control and CtIP depleted cells (P≥0.2). (C) Immunoblot analysis confirming knockdown of CtIP by two independent siRNAs in 3 independent experiments. Protein extracts were prepared at 48 hours post transfection. Blot was probed with anti-CtIP antibody as indicated on left. A Ku86 was used as a loading control. (D) BrdU incorporation is unaffected in CtIP depleted cells. siRNA transfected HeLa cells were synchronized with thymidine, were released into S-phase 48 hours post transfection, and fixed after 20 minutes BrdU incorporation. Cells were stained for BrdU. Left, Images of fixed control and CtIP depleted cells following staining for BrdU. Right, Quantification of relative BrdU signal in control and CtIP depleted cells.
CtIP is required for histone H2AX phosphorylation at laser-activated ICLs
To determine when CtIP acts in the ICL repair process, known markers of the DNA damage response and repair process were monitored in CtIP depleted HeLa cells. The first marker examined was γH2AX. To compare the function of CtIP in ICL repair to its known role at directly generated DSBs , , parallel experiments were conducted in which DSBS were generated directly by microirradiation with 532 nm laser light (64). Laser doses for 730 nm and 532 nm light were predetermined to use the minimal doses that give readily detectable γH2AX signals 2 hour post microirradiation. (Figure S2).
γH2AX phosphorylation was found to be strongly reduced in CtIP depleted S-phase HeLa cells along ICL containing microirradiated tracks (Figure 3A, top panel). In contrast, CtIP depletion had no detectable effect on H2AX phosphorylation at DSBs induced directly by laser irradiation (Figure 3A, bottom panel). The percentage of cells containing bright γH2AX signal, as determined by quantification of pixel intensity in individual cells along ICL containing laser tracks, was reduced significantly, over 4 fold, in cells depleted with 2 independent siRNAS targeting CtIP (13% and 19% respectively) relative to control cells (76%), (n = 48, 29 and 66 cells respectively; P-values = 0.003 (CtIP siRNA_1) and 0.009 (CtIP siRNA_2) (Figure 3B). In contrast, the percent cells with bright γH2AX along DSB containing laser tracks was not reduced in CtIP depleted cells (CtIP siRNA_1 82%, CtIP siRNA_2 94%) relative to control cells (85%), (n = 19, 19 and 26 cells respectively; P-value > = 0.5). The differential effects of CtIP depletion on H2AX phosphorylation at ICLs and DSBs suggests that CtIP plays a role in ICL repair that can be distinguished from its role in DSB repair.
(A) γH2AX staining of S-phase control and CtIP depleted cells 2 hours post microirradiation with 730 nm laser light in the presence of 8-MOP to form ICLs (above) or 532 nm laser light to form DSBs (below). (B) Quantification of cells scored as having bright γH2AX staining along laser tracks in control (light grey), CtIP siRNA_1(grey) and CtIP siRNA_2 (dark grey) depleted cells. Bars indicate standard deviation between 5 independent experiments.
To examine the function of CtIP relative to MUS81 and XPF, two nucleases that have been suggested to act early in ICL repair , , the effects of MUS81 and XPF depletion on γH2AX accumulation at ICLs was examined. Depletion of either XPF or MUS81 did not have a measurable effect on γH2AX accumulation along ICL containing laser tracks (Figure S3). This indicates that Mus81 and XPF function downstream of γH2AX generation in ICL repair.
CtIP is required for ATM phosphorylation at ICLs
ATM becomes activated in an MRN dependent manner and phosphorylates H2AX at DSBs early in DSB repair –, while ATR contributes to ATM activation and H2AX phosphorylation as a result of replication stress –. ATM has also been found to function in the FA pathway . To test if CtIP is required for ATM phosphorylation at ICLs, and thus functions upstream of DSB generation, we examined the effects of CtIP depletion on phosphorylation at serine-1981, a characterized autophosphorylation site. .
Consistent with the premise that DSBs are formed as an intermediate during ICL repair, ATM-pS1981 signal was readily detectable in control cells treated with 8-MOP and irradiated to form ICLs. In contrast, ATM-pS1981 signal along ICL containing laser tracks was reduced significantly in CtIP depleted S-phase HeLa cells (38%) relative to control cells (69%), (n = 32 and 27 cells respectively; P-value = 0.05) (Figure 4A, upper panel). By contrast, CtIP depletion did not significantly reduce the number of cells with bright ATM-pS1981 along DSBs (86%) relative to control cells (79%) (Figure 4A, lower panel), (n = 33 and 29 cells respectively; P-value > = 0.1) (Figure 4B).
(A) ATM-pS1981 staining of S-phase control and CtIP depleted cells 2 hours post microirradiation with 730 nm laser light in the presence of 8-MOP to form ICLs (top) or 532 nm laser light to form DSBs (below). (B) Quantification of cells scored as having bright ATM-pS1981 staining in control (light grey) CtIP siRNA_1(grey) and CtIP siRNA_2 (dark grey) depleted cells. Bars indicate standard deviation between 3 independent experiments.
CtIP is required for FANCD2 accumulation at ICLs
Biochemical analysis has demonstrated that the FANCI-FANCD2 complex is required for the incision of interstrand crosslinks in replication competent Xenopus extracts . We therefore examined whether FANCD2 was properly localized to laser activated ICLs in CtIP depleted cells. FANCD2 accumulation was found to be reduced along ICL containing microirradiated tracks in CtIP depleted cells (Figure 5A). The number of cells containing bright FANCD2 signal was reduced significantly by 2.7 fold in CtIP depleted cells (33%) relative to the control cells (88%) (n = 24 and 26 respectively; P-value = 0.026) (Figure 5B). These results demonstrate that CtIP acts upstream of FANCD2 localization to chromatin and point to a role for CtIP in ICL repair prior to ICL incision and unhooking.
(A) FANCD2 staining of S-phase control and CtIP depleted cells 2 hours post microirradiation with 730 nm laser light in the presence of 8-MOP. (B) Quantification of cells scored as having bright FANCD2 staining along laser tracks in control or CtIP depleted cells.
CtIP is required for RPA and ATR accumulation at ICLs
ATR phosphorylates the FANCI-FANCD2 complex which is required for its monoubiquitination and localization to ICLs . RPA coated ssDNA is required for ATR activation  and CtIP/MRN is required for resection at double strand breaks , . We hypothesized that CtIP might facilitate resection of DNA ends present at an ICL stalled replication fork. Therefore we examined RPA2 accumulation at ICL containing microirradiated tracks in CtIP depleted cells compared to control cells. RPA2 accumulation at laser tracks was found to be strongly reduced in CtIP depleted S-phase HeLa (Figure 6A). The percent cells containing bright RPA2 tracks was reduced 2.7 fold in CtIP depleted cells (27%) relative to control cells (73%) (n = 29 and 41 cells respectively, P value = 0.005) (Figure 6B).
(A) RPA staining of S-phase control and CtIP depleted cells 2 hours post microirradiation with 730 nm laser light in the presence of 8-MOP. (B) Quantification of cells scored as having bright RPA staining intensity along laser tracks in control or CtIP depleted cells. (C) GFP-CtIP or GFP-CtIPT847A in S-phase cells pre pre-and post-microirradiation with 730 nm light in the presence of 8-MOP. Cells were stained for RPA2. (D) Quantification of RPA2 along laser tracks in cells scored positive for GFP-CtIP or GFP-CtIPT847A accumulation. (E) ATR staining of S-phase control and CtIP depleted cells 2 hours post microirradiation with 730 nm laser light in the presence of 8-MOP. (F) Quantification of cells scored as having bright ATR staining along laser tracks in control or CtIP depleted cells. Bars indicate standard deviation between 3 independent experiments.
CtIP is targeted for phosphorylation at Thr847 by cyclin dependent kinase (CDK) . Phosphorylation at this site is required to promote resection at DSBs, but is not required for CtIP recruitment to DSBs , . We tested whether a Thr-847 to Ala CtIP mutation would also affect resection at ICLs. Endogenous CtIP was depleted by siRNA and replaced by either wildtype GFP-CtIP or GFP-CtIPT847A in U2OS cells. HeLa were found to be sensitive to increased levels of CtIP, therefore we used U2OS cells for experiments involving ectopic expression of CtIP. U2OS cells were shown to react similarly to CtIP depletion compared to HeLa cells (Figure S4). S-phase cells were irradiated to form ICLs and stained for RPA2. GFP-CtIPT847A accumulated at ICL containing laser tracks comparable to wildtype levels, however RPA2 accumulation was impaired relative to cells expressing wildtype GFP-CtIP (Figure 6C). The percent cells containing bright RPA2 tracks was reduced 7.9 fold in cells expressing the CtIP phosphorylation mutant (8%) relative to control cells (63%) (n = 20 and 20 cells respectively, P value = 0.03) (Figure 6D).
We next examined whether reduced RPA accumulation at ICLs in CtIP depleted cells was associated with reduced ATR recruitment. The percent cells containing bright ATR signal along ICL containing laser tracks was reduced over 7 fold in CtIP depleted cells (8%) relative to control cells (58%) (n = 24 and 34 cells respectively; P value = 0.003) (Figure 6E, 6F). The requirement of CtIP for both RPA and ATR localization to ICL containing chromatin suggests that CtIP acts early in ICL repair prior to ssDNA generation and ICL incision.
BRCA1 is required for CtIP accumulation at ICLs
BRCA1 ubiquitinates CtIP and is required for its localization to DSBs , . In order to further characterize the requirements for CtIP recruitment to ICLs we examined whether BRCA1 was required for GFP-CtIP accumulation at ICLs. Cells were either BRCA1 depleted using two previously described independent siRNAs ,  or treated with control siRNA. Endogenous CtIP was depleted by siRNA and CtIP expression reconstituted with silencing resistant GFP-CtIP. GFP-CtIP accumulation at ICL containing laser tracks was examined in S phase siRNA treated cells. CtIP accumulation at ICLs was found to be dependent on the presence of BRCA1 (Figure 7). In 3 independent experiments all cells (>25) treated with BRCA1 siRNA that lacked visible BRCA1 expression as verified by immunofluorescence staining and imaging, did not contain visible GFP-CtIP along the micro-irradiated region. In contrast, all control siRNA treated cells (>25) that had robust BRCA1 expression levels also contained GFP-CtIP at the ICL containing laser tracks. These results demonstrate that BRCA1 is required for CtIP recruitment to ICLs.
GFP-CtIP in S-phase control and BRCA1 depleted cells pre-and post-microirradiation with 730 nm light in the presence of 8-MOP.
CtIP is recruited to ICLs in a FANCM–dependent manner
FANCM has been shown to be required for RPA loading at ICLs as well as for activating the S-phase checkpoint , . Data presented in Figure 6 indicates that CtIP is required for both RPA and ATR accumulation at laser activated ICLs in replicating cells. In order to determine when CtIP acts relative to FANCM we examined whether FANCM is required for CtIP localization to ICLs. U2OS cells stably expressing GFP-CtIP in which endogenous CtIP is depleted were treated with two independent FANCM siRNA s or control siRNA. Depletion was confirmed by immunoblot (Figure 8A). Cells were microirradiated to form ICLs and CtIP accumulation was examined. The percent of cells containing GFP-CtIP along ICL containing laser tracks was significantly reduced in FANCM depleted cells (22% FANCM siRNA_1, 0% FANCM siRNA_2) relative to control cells (67%) (n = 26, 11 and 30 cells respectively; P value = 0.0002) (Figure 8B, 8C). Next we examined whether FANCM was required for GFP-CtIP recruitment to DSBs. Cells treated with FANCM siRNA_2 or control siRNA were irradiated with 532 nm light to form DSBs and GFP-CtIP localization was monitored. In contrast to what was observed at ICLs, FANCM depletion did not have a significant effect on the percent of cells containing GFP-CtIP at DSB containing laser tracks (75% FANCM siRNA_2) relative to control cells (76%)(n = 20 and 17 cells respectively) (Figure 8D, 8E). This data suggests that FANCM acts upstream of CtIP and is required for its localization to ICL but not DSB containing chromatin.
(A) Immunoblot of control cells and cells depleted for FANCM. (B) GFP-CtIP in S-phase control and FANCM depleted cells pre-and post-microirradiation with 730 nm light in the presence of 8-MOP. (C) Quantification of cells scored as having visible GFP-CtIP along laser tracks in control or depleted cells. Bars indicate standard deviation between 3 independent experiments. (D) GFP-CtIP in S-phase control and FANCM depleted cells pre- and post-microirradiation with green laser to generate DSBs. (E) Quantification of cells scored as having bright GFP-CtIP along DSB containing laser tracks. (F) Model of CtIP function in replication associated ICL repair. FANCM binds ICL stalled replication fork and remodels fork to enable CtIP and MRN access. BRCA1 ubiquitinates CtIP facilitating its localization to damaged chromatin. CtIP and MRN act to generate ssDNA at a stalled fork. RPA bound single stranded DNA activates ATR. ATR phosphorylates FANCD2 followed by FA core complex ubiquitination of the FANCI-FANCD2 complex. The monoubiquitinated FANCI-FANCD2 complex localizes to the damaged chromatin and facilitates ICL incision and downstream repair events. CtIP and MRN act again to resect ends, activate ATM, facilitate completion of repair by homologous recombination.
The cellular response to ICLs involves the intersection of the DNA repair and replication checkpoint pathways. The FANCM/FAAP24 complex binds to, remodels and stabilizes stalled replication forks at an early step in ICL repair , . FANCM/FAAP24 is also required for ATR mediated checkpoint activation in response to ICL stalled replication forks , . In addition, FANCM deficient cells have decreased levels of FANCD2 monoubiquitination and chromatin bound FANCD2 , , . We have shown that FANCM is required for CtIP localization to ICLs in replicating cells. CtIP in turn is required for proper accumulation of RPA, ATR and FANCD2 at ICLs. This places CtIP within the initiating steps of ICL repair, downstream of FANCM and upstream of RPA (Figure 8F). We propose the following model. First, FANCM/FAAP24 remodels ICL stalled replication forks to enable CtIP access. BRCA1 interacts with and ubiquitinates CtIP enabling it to bind to the damaged chromatin. Next, CtIP, presumably in concert with MRN, supports initiation of resection of the lagging strands of the previously active replication fork , , . This resection activity is dependent on CDK phosphorylation site T847 on CtIP. ssDNA-RPA provides a platform for ATR-ATRIP binding. Once localized to the stalled fork activated ATR promotes S phase checkpoint activation and phosphorylates the FANCI-FANCD2 complex. The phosphorylated FANCI-FANCD2 complex is then monoubiquitinated, localized to damaged chromatin to facilitate ICL incision and generation of a DSB repair intermediate. This proposed order of events is consistent with that described for Xenopus extracts in which replication dependent ICL repair initiates at an ICL stalled fork, followed by generation of ssDNA, activation of ATR as measured by Chk1 phosphorylation, and excision of the crosslink in a FANCI-FANCD2 dependent manner , .
Cell cycle distribution and rate of BrdU incorporation are unaffected in CtIP depleted HeLa cells compared to control cells. This suggests that ICL processing defects observed in CtIP depleted cells are due to a deficiency in initiation of repair as opposed to an inhibition of cell cycle progression. The difference observed in cell cycle distribution of our CtIP depleted cells compared to those observed in mouse fibroblasts  are likely due to a difference in cell type as well as to a difference in the timing and method used to deplete CtIP.
A function for CtIP prior to ICL incision, and upstream of a repair intermediate that contains double stranded ends, is supported by the observation that CtIP depleted cells show a striking reduction in the accumulation of the DSB markers ATM-pS1981 and γH2AX at laser generated ICL tracks. In contrast, the accumulation of ATM-pS1981 and γH2AX at DSBs produced by direct laser irradiation are not affected by CtIP depletion. The effect of CtIP depletion on γH2AX at DSBs is in agreement with previously published observations in CtIP depleted U2OS cells . This indicates that initiation of DSB repair, is not grossly affected by CtIP depletion. These results do not preclude an additional downstream role for CtIP where it may act together with MRN in a manner analogous to its function at directly generated DSBs to facilitate the processing of the double stranded DNA ends produced following ICL incision.
In summary, our data supports a model in which CtIP functions early in replication associated ICL repair downstream of FANCM and is required for the accumulation of RPA, ATR, FANCD2, ATM-pS1981, and γH2AX at ICLs. Thus, CtIP plays a critical role in initiating the DNA damage response at ICL stalled replication forks, prior to the generation of a double stranded DNA repair intermediate. It will be of interest to see how CtIP and MRN are regulated at ICL stalled forks and whether this response is different from that observed at other stalled forks in which helicase uncoupling contributes to checkpoint activation.
Materials and Methods
Robolase III (RLIII) is a multi-modality laser ablation system that is based on a femtosecond pulsed Ti:Sapphire laser (Mai Tai, Spectraphysics, Newport Corp., Mountain view, CA) and a motorized inverted microscope (Axiovert 200 M, Zeiss) that utilizes a custom Labview-based software package developed specifically for the Robolase series of microscope systems . In this study, the laser wavelength was set to 730 nm. The effective wavelength at the focal point is 365 nm at which psoralen is activated by a 2-photon mechanism . The pulse duration was estimated at 200 fs and the repetition rate was 76 MHz. The laser was focused by a Zeiss 63×/1.4 plan-apochromat PH3 oil objective with measured transmission of 67% at 730 nm using the double-objective method to determine transmission . The power used in this study was 2 mW before the objective which yielded a peak irradiance of 2.8×1010 W/cm2 at the focal point. For each cell, a 10 µm by 636 nm region of interest (ROI) was chosen inside the nucleus using real-time phase contrast imaging. An image of the designated ROI was recorded as reference. Laser exposure over each 10 µm long ROI was performed four times over each ROI with a total energy of 2.4 mJ. H2AX phosphorylation was used as a marker to determine the minimum power that provided a signal in the presence of 8-MOP. Double strand breaks were generated with the Robolase II (RLII) system that uses a frequency doubled 532 nm12 ps pulsed Nd:YVO4 laser , . The ROI for each cell was 10 µm by 464 nm. The laser power used in this study was 5 mW in the focal spot for an irradiance of 2.3×109 W/cm2 and the total energy deposited along the laser track inside each cell was 3.2 mJ. For experiments in which DSBs were generated cells were laser microirradiated on the same dish as cells treated to form ICLs and fixed at 2 hours 10 minutes post laser.
Cell culture, siRNA transfection, and survival assays
Asynchronous or rapidly proliferating HeLa and HEK293 cells were maintained in Dulbecco's modified Eagle's medium (Invitrogen, Carlsbad, CA) supplemented with 10% bovine calf serum L-glutamine, and sodium pyruvate) at 37°C and 5% CO2.
Small interfering double stranded RNAs (siRNAs) were introduced into HeLa cells by transfecting cells in a 6 well dish with 50 pmol siRNA, and 5 µL Dharmafect 1 (Dharmacon, Lafayette, CO) per reaction. The following synthetic siRNAs used were obtained from Dharmacon, siLuciferase (control) and CtIP (siCtIP_1 and siCtIP_2) , FANCM_1 (GCAAAGUAGCCUAAAGAAAUU), FANCM_2 , siMUS81 (D-016043) and siRNA pool containing 4 siRNAs targeting XPF (siERCC4 D-019946-01.) The following siRNAs were obtained from Integrated DNA Technologies, BRCA1_1 (AATGCCAAAGTAGCTAATGTAUU)  and BRCA1_3 (AAGGAACCUGUCUCC ACA AAG UU) .
HEK293 cells were transfected with the indicated siRNA using Dharmafect 1, sixteen hours later the cells were washed with sterile PBS and fresh media was added. After an eight hour recovery the cells were trypsinized and seeded at 104 per well in a six well plate. After 12 hours 10 µg/ml 8-MOP or angelicin were added to the cells. After 30 minutes incubation the cells were then exposed to the indicated amount of UVA radiation at approximately 360 nm using a Stratalinker (Stratagene, La Jolla, CA). Alternatively, cells were treated with indicated amount of MMC for 2 hours. Post treatment the cells were washed with sterile PBS, fresh media added and replaced every three days. On day 8 the cells were trypsinized and viable cells were counted using a CASY cell counter (Scharfe systems).
GFP-CtIP expressing cells
A retroviral expression vector containing EGFP-CtIP (pBabepuro) was infected into U2OS cells for 48 hrs, followed by puromycin selection for 2–3 days to generate stable cell lines. For transient expression endogenous CtIP was first depleted by transfecting CtIP siRNA_1 into cells. Cells were transfected 24 hours later with silencing resistant GFP-CtIP using Effectene (Qiagen). Experiments were performed 24 hours post GFP-CtIP transfection. GFP-CtIPT847A was generated using Quikchange Site Directed Mutagenesis Kit (Agilent Technologies).
Total RNA was isolated from control or CtIP siRNA transfected cells 48 hours post transfection using the RNeasy Kit (Qiagen). Target RNA was amplified using the Bio-rad iScript One Step RT-PCR kit with SYBR green kit (Bio-rad, Hercules, CA) on a Bio-rad real time quantitative PCR machine. The One step kit was used according to manufacturer's directions with the exception of 20 µL reactions, 2 ng total RNA per reaction, and 2 µL of each primer (5 uM stock). The following primers were used, housekeeping gene PBGD was amplified as a control (PBGDF- TCC AAG CGG AGC CAT GTC TG, PBGDR- AGAATC TTG TCC CCT GTG GTG GA) CtIP (CTIPF- AAG AGG AGG AAT TGT CTA CTG C, CTIPR- AGA ATC TTG TCC CCT GTG GTG GA). Reactions were run on Chromo-4 qPCR I system (MJ Research, Waltham, MA). CtIP RNA depletion was verified to be between 60 and 70% by RT-QPCR for CtIP siRNA 1 and CtIP siRNA 2 in all experiments relative to control depleted cells.
Bromodeoxyuridine incorporation assay
HeLa cells were transfected with siRNA as described above and seeded onto coverslips in 12-well plates. Thirty-six hours later, 2 mM thymidine was added to cultures for 16 hours. Cells were released from the thymidine block by washing 2 times with fresh media containing 100 uM bromodeoxyuridine (BrdU). Cells were incubated in BrdU containing media for 20 minutes to label S phase nuclei.. Cultures were fixed with 3.7% formaldehyde, stained with mouse monoclonal anti-BrdU antibody coupled to FITC (eBioscience, San Diego, CA), and counterstained with DAPI. ImageJ software was used to determine the total number of nuclei, BrdU-positive nuclei, and relative levels of fluorescence in individual cells.
Cell cycle analysis
siRNA and control cells were prepared for flow cytometry analysis 48 hours post transfection. Cells were treated with trypsin/EDTA and washed twice in PBS before fixing them in 70% ethanol overnight at −20°C. Cells were then washed twice in PBS and incubated in staining solution (20 µg/ml propidium iodide, 20 µg/ml RNase A, 0.1% Triton X-100 in PBS) for 30 min at 37°C.Data were acquired on a BD FACS Calibur flow cytometer. Percentages of G1, S, and G2 phase cells were determined from cell cycle profiles by using the Watson pragmatic algorithm of the cell cycle platform within FlowJo software (Tree Star Inc., Ashland, OR) with the “remove doublets” and “remove debris” options enabled. P values were determined using an unpaired two-tailed t test.
Cells for laser microirradiation were cultured on gridded glass bottom dishes (Mattek, Ashland, MA) for 16 hours in 2 mM thymidine. Cells were washed twice with warm media to remove thymidine one hour prior to microirradiation and fresh media was added. Twenty minutes prior to laser microirradiation drugs were added to the cells; 10 µg/ml 8-MOP (MP Biomedicals, Solon, Ohio), or an equivalent molar amount of angelicin (8.6 µg/ml Sigma-Aldrich, St. Louis, MO).
Cells were allowed to recover for 2 hours post micoirradiation prior to fixation in all experiments except where noted. Soluble proteins were extracted in cytoskeletal buffer on ice for 5 minutes (10 mM Pipes pH6.8, 100 mM NaCl, 300 mM sucrose, 3 mM MgCl2, 1 mM EDTA and 0.5% TritonX-100) , followed by fixation in 3.7% formaldehyde phosphate buffered saline (PBS) at room temperature for 10 minutes, and permeabilized with 0.2% Triton-X. Cells were then stained with primary antibody in 3% BSA/PBS. The following primary antibodies were used in immunofluorescent staining: 1:100 rabbit anti-RAD51 1:100 (Abcam, Cambridge, MA), 1:1000 mouse anti-γH2AX (Upstate Biotechnology, Waltham, MA), 1:250 Rabbit anti-NBS1 NB100-143 (Novus Biologicals, Littleton, CO), 1:200 Mouse anti ATM-pS1981 clone 10H11.E12 (Chemicon, Billerica, MA), 1:200 Rabbit anti-FANCD2 NB100-182 (Novus Biologicals, Littleton, CO), 1:50 Mouse Anti-RPA2 (Calbiochem, Gibbstown, NJ), 1:100 Mouse anti-BrdU (ebioscience, San Diego, CA), 1:500 Rabbit anti-RAD51 H92 sc-8349 (Santa Cruz Biotechnology, Santa Cruz, CA), 1:1000 Mouse anti-MUS81 ab14387 (Abcam), 1:500 XPF Ab17798 (Abcam), 1:500 Rabbit anti-BRCA1 PA1-14072 (Thermo Fisher) 1:1000 Rabbit anti-Ku86 SC9034 (Santa Cruz Biotechnology, Santa Cruz, CA). The following secondary antibodies were used at a 1:5000 dilution in 3%BSA/PBS 1:5000 Alexa Fluor 488 goat anti-mouse IgG (Molecular Probes, Eugene, OR) and 1:5000 Alexa Fluor 594 goat anti-rabbit IgG (Molecular Probes, Eugene, OR). Nuclei were visualized by staining with 1 µg/ml Dapi (Invitrogen). Glass coverslips were mounted with Vectashield (Vectorlabs, Burlingham, CA). Samples were visualized and images acquired using a 63× objective on a Leica DM IRE2 microscope equipped with a Hamamatsu C4742-95 digital charge-coupled-device camera.
Quantification of immunofluorescence
Images of cells were analyzed using Image J software (NIH, Bethesda, MD). The fluorescence along the microirradiated track was quantified in each individual cell as follows. Images were thresholded and converted into binary images. The same threshold was applied to all images from a single experiment. The number of pixels above threshold in 3 oval ROIs (150×50 pixels) were acquired per cell: one measurement for the area containing the laser track, and two measurements to determine the level of background signal in the nuclear region outside the laser track. The average number of background pixels was subtracted from the number of pixels measured along the microirradiated track for each individual cell. This resulted in a corrected pixel number for the intensity of a fluorescent signal along a laser track. For each positive control the average pixel number along the laser track was determined similarly. The average value from the positive control group per experiment was used to define the cut-off for experimental signals designated “bright” (corrected pixel number >50% of average positive control) or “low” (corrected pixel number <50% of average positive control). Each cell in the control and experimental siRNA group was then assigned a low signal or bright signal accordingly. The number of cells that fell into the “bright” and “low” categories were determined for each experiment. Cells which did not contain pan-nuclear γH2AX or RPA2 foci were considered to be outside of S-phase and were excluded from analysis. For analysis of GFP-CtIP expressing cells, cells were scored as positive if there was any detectable GFP-CtIP along laser track.
Statistical analysis was performed using Microsoft Excel. Differences between control and experimental groups were considered statistically significant when the P-value, determined by a two-tailed unpaired Student's t-test, was ≤0.05.
HeLa cells were lysed (10 mM Hepes pH 7.9, 10 mM KCl, 1.5 mM MgCl2, 0.34 M sucrose, 10% glycerol, 1 mM DTT, 0.1% triton, and protease inhibitors). Nuclear fraction was harvested by centrifugation at 1,399×g for 5 minutes. Pellet was resuspended in loading buffer, boiled for 5 mintues and put through 25 gauge syringe. Proteins were resolved by SDS-PAGE and transferred to nitrocellulose. Immunoblots were probed with indicated primary antibody, anti-FANCM (1:1000) ab35620 (Abcam) and anti-Ku86 (1:1000) (Santa Cruz). R. Baer provided a mouse monoclonal antibody to CtIP . Membranes were washed, incubated with HRP-linked secondary antibodies (Invitrogen), and detected by chemiluminescence (Pierce, Fisher Scientific). For Mus81 and XPF blots cells were lysed by boiling in Laemmli buffer (4% SDS, 10% glycerol, 62.5 mM Tris pH6.8, 10% β-mercaptoethanol), and sonicated on ice. Immunoblots were probed with indicated primary antibody, anti-MUS81 (1:1000) (Abcam) and anti-XPF (1:1000) (Abcam), and anti-Ku86 (1:1000) (Santa Cruz).
Effect of CtIP depletion on IR sensitivity. Survival of HEK293 cells transfected with control or CtIP siRNAs and exposed to IR. CtIP_1 and CtIP_2 are two independent siRNAs. Cells were irradiated 48 hours post transfection and survival was assessed 8 days post irradiation. Fraction surviving cells is calculated in respect to untreated cells.
Timecourse of γH2AX and RAD51 appearance at ICLs and DSBs. (A) S-phase, 8-MOP treated cells were fixed and stained for γH2AX and Rad51 at indicated times post microirradiation with 730 nm laser light. B, Cells were microirradiated with 532 nm laser light to generate double strand breaks. Cells were fixed and stained for γH2AX and Rad51 at indicated times post microirradiation. *Time point used in experiments.
MUS81 and XPF depletion do not affect H2AX phosphorylation at ICLs. (A) Left, γH2AX staining of S-phase control and MUS81 depleted cells 2 hours post microirradiation with 730 nm laser light in the presence of 8-MOP. Right, Quantification of γH2AX staining intensity along laser tracks in control (light grey) and Mus81 depleted cells (dark grey) microirradiated to form ICLs. Bar graph indicates percentage of total cells scored as having bright γH2AX signal along laser tracks. More than 30 cells were analyzed per condition. Bars indicate standard deviation between 3 independent experiments. (B) Left, γH2AX staining of S-phase control and XPF depleted cells 2 hours post microirradiation with 730 nm laser light in the presence of 8-MOP. Right, Quantification of γH2AX staining intensity along laser tracks in control (light grey) and XPF depleted cells (dark grey) microirradiated to form ICLs. Bar graph indicates percentage of total cells scored as having bright γH2AX signal along laser tracks. Bars indicate standard deviation. (C) Immunoblot confirmation of knockdown efficiency of MUS81 and XPF siRNAs. Ku86 is loading control.
CtIP depletion in U2OS cells reduces γH2AX at ICLs. (A) γH2AX staining of S-phase control and CtIP depleted cells 2 hours post microirradiation with 730 nm laser light in the presence of 8-MOP. (B) γH2AX staining of cell treated with CtIP siRNA and complemented with GFP-CtIP expression. (C) Quantification of γH2AX staining intensity along laser tracks in control, CtIP depleted, and CtIP depleted and GFP-CtIP complemented cells. Bar graph indicates percentage of total cells scored as having bright γH2AX signal along laser tracks (Over 15 cells were scored for each condition).
CtIP antibodies were kindly provided by R. Baer (Columbia University). We thank S. Jackson (University of Cambridge) for providing the silencing resistant GFP-CtIP construct. We thank Larry Gerace and Michael Huber (The Scripps Research Institute) for help with microscopy, Paul Russell (The Scripps Research Institute) for helpful discussions, and Xiaohua Wu (The Scripps Research Institute) for providing U2OS stable lines expressing GFP-CtIP .
Conceived and designed the experiments: MLD MWB CHM. Performed the experiments: MLD QZ ERT AJT. Analyzed the data: MLD ERT CHM. Contributed reagents/materials/analysis tools: QZ LZS MWB. Wrote the paper: MLD CHM.
- 1. D'Andrea AD (2010) Susceptibility pathways in Fanconi's anemia and breast cancer. N Engl J Med 362: 1909–1919. doi: 10.1056/nejmra0809889
- 2. Andreassen PR, Ren K (2009) Fanconi anemia proteins, DNA interstrand crosslink repair pathways, and cancer therapy. Curr Cancer Drug Targets 9: 101–117. doi: 10.2174/156800909787314011
- 3. McVey M (2010) Strategies for DNA interstrand crosslink repair: insights from worms, flies, frogs, and slime molds. Environ Mol Mutagen 51: 646–658. doi: 10.1002/em.20551
- 4. Akkari YM, Bateman RL, Reifsteck CA, Olson SB, Grompe M (2000) DNA replication is required To elicit cellular responses to psoralen-induced DNA interstrand cross-links. Mol Cell Biol 20: 8283–8289. doi: 10.1128/mcb.20.21.8283-8289.2000
- 5. Rothfuss A, Grompe M (2004) Repair kinetics of genomic interstrand DNA cross-links: evidence for DNA double-strand break-dependent activation of the Fanconi anemia/BRCA pathway. Mol Cell Biol 24: 123–134. doi: 10.1128/mcb.24.1.123-134.2004
- 6. Sobeck A, Stone S, Costanzo V, de Graaf B, Reuter T, et al. (2006) Fanconi anemia proteins are required to prevent accumulation of replication-associated DNA double-strand breaks. Mol Cell Biol 26: 425–437. doi: 10.1128/mcb.26.2.425-437.2006
- 7. Mladenova V, Russev G (2006) Enhanced repair of DNA interstrand crosslinks in S phase. FEBS Lett 580: 1631–1634. doi: 10.1016/j.febslet.2006.02.009
- 8. McHugh PJ, Sarkar S (2006) DNA interstrand cross-link repair in the cell cycle: a critical role for polymerase zeta in G1 phase. Cell Cycle 5: 1044–1047. doi: 10.4161/cc.5.10.2763
- 9. Muniandy PA, Thapa D, Thazhathveetil AK, Liu ST, Seidman MM (2009) Repair of laser-localized DNA interstrand cross-links in G1 phase mammalian cells. J Biol Chem 284: 27908–27917. doi: 10.1074/jbc.m109.029025
- 10. Ben-Yehoyada M, Wang LC, Kozekov ID, Rizzo CJ, Gottesman ME, et al. (2009) Checkpoint signaling from a single DNA interstrand crosslink. Mol Cell 35: 704–715. doi: 10.1016/j.molcel.2009.08.014
- 11. Raschle M, Knipscheer P, Enoiu M, Angelov T, Sun J, et al. (2008) Mechanism of replication-coupled DNA interstrand crosslink repair. Cell 134: 969–980. doi: 10.1016/j.cell.2008.08.030
- 12. Ciccia A, Ling C, Coulthard R, Yan Z, Xue Y, et al. (2007) Identification of FAAP24, a Fanconi anemia core complex protein that interacts with FANCM. Mol Cell 25: 331–343. doi: 10.1016/j.molcel.2007.01.003
- 13. Gari K, Decaillet C, Delannoy M, Wu L, Constantinou A (2008) Remodeling of DNA replication structures by the branch point translocase FANCM. Proc Natl Acad Sci U S A 105: 16107–16112. doi: 10.1073/pnas.0804777105
- 14. Deans AJ, West SC (2009) FANCM connects the genome instability disorders Bloom's Syndrome and Fanconi Anemia. Mol Cell 36: 943–953. doi: 10.1016/j.molcel.2009.12.006
- 15. Huang M, Kim JM, Shiotani B, Yang K, Zou L, et al. (2010) The FANCM/FAAP24 complex is required for the DNA interstrand crosslink-induced checkpoint response. Mol Cell 39: 259–268. doi: 10.1016/j.molcel.2010.07.005
- 16. Schwab RA, Blackford AN, Niedzwiedz W (2010) ATR activation and replication fork restart are defective in FANCM-deficient cells. EMBO J 29: 806–818. doi: 10.1038/emboj.2009.385
- 17. Singh TR, Saro D, Ali AM, Zheng XF, Du CH, et al. (2010) MHF1-MHF2, a histone-fold-containing protein complex, participates in the Fanconi anemia pathway via FANCM. Mol Cell 37: 879–886. doi: 10.1016/j.molcel.2010.01.036
- 18. Knipscheer P, Raschle M, Smogorzewska A, Enoiu M, Ho TV, et al. (2009) The Fanconi anemia pathway promotes replication-dependent DNA interstrand cross-link repair. Science 326: 1698–1701. doi: 10.1126/science.1182372
- 19. Zou L, Elledge SJ (2003) Sensing DNA damage through ATRIP recognition of RPA-ssDNA complexes. Science 300: 1542–1548. doi: 10.1126/science.1083430
- 20. Andreassen PR, D'Andrea AD, Taniguchi T (2004) ATR couples FANCD2 monoubiquitination to the DNA-damage response. Genes Dev 18: 1958–1963. doi: 10.1101/gad.1196104
- 21. Pichierri P, Rosselli F (2004) The DNA crosslink-induced S-phase checkpoint depends on ATR-CHK1 and ATR-NBS1-FANCD2 pathways. EMBO J 23: 1178–1187. doi: 10.1038/sj.emboj.7600113
- 22. Byun TS, Pacek M, Yee MC, Walter JC, Cimprich KA (2005) Functional uncoupling of MCM helicase and DNA polymerase activities activates the ATR-dependent checkpoint. Genes Dev 19: 1040–1052. doi: 10.1101/gad.1301205
- 23. Long DT, Raschle M, Joukov V, Walter JC (2011) Mechanism of RAD51-dependent DNA interstrand cross-link repair. Science 333: 84–87. doi: 10.1126/science.1204258
- 24. Ho GP, Margossian S, Taniguchi T, D'Andrea AD (2006) Phosphorylation of FANCD2 on two novel sites is required for mitomycin C resistance. Mol Cell Biol 26: 7005–7015. doi: 10.1128/mcb.02018-05
- 25. Ishiai M, Kitao H, Smogorzewska A, Tomida J, Kinomura A, et al. (2008) FANCI phosphorylation functions as a molecular switch to turn on the Fanconi anemia pathway. Nat Struct Mol Biol 15: 1138–1146. doi: 10.1038/nsmb.1504
- 26. Garcia-Higuera I, Taniguchi T, Ganesan S, Meyn MS, Timmers C, et al. (2001) Interaction of the Fanconi anemia proteins and BRCA1 in a common pathway. Mol Cell 7: 249–262. doi: 10.1016/s1097-2765(01)00173-3
- 27. Smogorzewska A, Matsuoka S, Vinciguerra P, McDonald ER 3rd, Hurov KE, et al. (2007) Identification of the FANCI protein, a monoubiquitinated FANCD2 paralog required for DNA repair. Cell 129: 289–301. doi: 10.1016/j.cell.2007.03.009
- 28. Alpi AF, Pace PE, Babu MM, Patel KJ (2008) Mechanistic insight into site-restricted monoubiquitination of FANCD2 by Ube2t, FANCL, and FANCI. Mol Cell 32: 767–777. doi: 10.1016/j.molcel.2008.12.003
- 29. Niedernhofer LJ, Odijk H, Budzowska M, van Drunen E, Maas A, et al. (2004) The structure-specific endonuclease Ercc1-Xpf is required to resolve DNA interstrand cross-link-induced double-strand breaks. Mol Cell Biol 24: 5776–5787. doi: 10.1128/mcb.24.13.5776-5787.2004
- 30. Al-Minawi AZ, Lee YF, Hakansson D, Johansson F, Lundin C, et al. (2009) The ERCC1/XPF endonuclease is required for completion of homologous recombination at DNA replication forks stalled by inter-strand cross-links. Nucleic Acids Res 37: 6400–6413. doi: 10.1093/nar/gkp705
- 31. Bhagwat N, Olsen AL, Wang AT, Hanada K, Stuckert P, et al. (2009) XPF-ERCC1 participates in the Fanconi anemia pathway of cross-link repair. Mol Cell Biol 29: 6427–6437. doi: 10.1128/mcb.00086-09
- 32. Fekairi S, Scaglione S, Chahwan C, Taylor ER, Tissier A, et al. (2009) Human SLX4 is a Holliday junction resolvase subunit that binds multiple DNA repair/recombination endonucleases. Cell 138: 78–89. doi: 10.1016/j.cell.2009.06.029
- 33. Crossan GP, van der Weyden L, Rosado IV, Langevin F, Gaillard PH, et al. (2011) Disruption of mouse Slx4, a regulator of structure-specific nucleases, phenocopies Fanconi anemia. Nat Genet doi: 10.1038/ng.752
- 34. Kim Y, Lach FP, Desetty R, Hanenberg H, Auerbach AD, et al. (2011) Mutations of the SLX4 gene in Fanconi anemia. Nat Genet doi: 10.1038/ng.750
- 35. Stoepker C, Hain K, Schuster B, Hilhorst-Hofstee Y, Rooimans MA, et al. (2011) SLX4, a coordinator of structure-specific endonucleases, is mutated in a new Fanconi anemia subtype. Nat Genet doi: 10.1038/ng.751
- 36. Yamamoto KN, Kobayashi S, Tsuda M, Kurumizaka H, Takata M, et al. (2011) Involvement of SLX4 in interstrand cross-link repair is regulated by the Fanconi anemia pathway. Proc Natl Acad Sci U S A 108: 6492–6496. doi: 10.1073/pnas.1018487108
- 37. Wang AT, Sengerova B, Cattell E, Inagawa T, Hartley JM, et al. (2011) Human SNM1A and XPF-ERCC1 collaborate to initiate DNA interstrand cross-link repair. Genes Dev 25: 1859–1870. doi: 10.1101/gad.15699211
- 38. Hazrati A, Ramis-Castelltort M, Sarkar S, Barber LJ, Schofield CJ, et al. (2008) Human SNM1A suppresses the DNA repair defects of yeast pso2 mutants. DNA Repair (Amst) 7: 230–238. doi: 10.1016/j.dnarep.2007.09.013
- 39. Bae JB, Mukhopadhyay SS, Liu L, Zhang N, Tan J, et al. (2008) Snm1B/Apollo mediates replication fork collapse and S Phase checkpoint activation in response to DNA interstrand cross-links. Oncogene 27: 5045–5056. doi: 10.1038/onc.2008.139
- 40. Hanada K, Budzowska M, Modesti M, Maas A, Wyman C, et al. (2006) The structure-specific endonuclease Mus81-Eme1 promotes conversion of interstrand DNA crosslinks into double-strands breaks. EMBO J 25: 4921–4932. doi: 10.1038/sj.emboj.7601344
- 41. Ciccia A, McDonald N, West SC (2008) Structural and functional relationships of the XPF/MUS81 family of proteins. Annu Rev Biochem 77: 259–287. doi: 10.1146/annurev.biochem.77.070306.102408
- 42. Dendouga N, Gao H, Moechars D, Janicot M, Vialard J, et al. (2005) Disruption of murine Mus81 increases genomic instability and DNA damage sensitivity but does not promote tumorigenesis. Mol Cell Biol 25: 7569–7579. doi: 10.1128/mcb.25.17.7569-7579.2005
- 43. Taylor ER, McGowan CH (2008) Cleavage mechanism of human Mus81-Eme1 acting on Holliday-junction structures. Proc Natl Acad Sci U S A 105: 3757–3762. doi: 10.1073/pnas.0710291105
- 44. Kratz K, Schopf B, Kaden S, Sendoel A, Eberhard R, et al. (2010) Deficiency of FANCD2-associated nuclease KIAA1018/FAN1 sensitizes cells to interstrand crosslinking agents. Cell 142: 77–88. doi: 10.1016/j.cell.2010.06.022
- 45. MacKay C, Declais AC, Lundin C, Agostinho A, Deans AJ, et al. (2010) Identification of KIAA1018/FAN1, a DNA repair nuclease recruited to DNA damage by monoubiquitinated FANCD2. Cell 142: 65–76. doi: 10.1016/j.cell.2010.06.021
- 46. Smogorzewska A, Desetty R, Saito TT, Schlabach M, Lach FP, et al. (2010) A genetic screen identifies FAN1, a Fanconi anemia-associated nuclease necessary for DNA interstrand crosslink repair. Mol Cell 39: 36–47. doi: 10.1016/j.molcel.2010.06.023
- 47. Niedzwiedz W, Mosedale G, Johnson M, Ong CY, Pace P, et al. (2004) The Fanconi anaemia gene FANCC promotes homologous recombination and error-prone DNA repair. Mol Cell 15: 607–620. doi: 10.1016/j.molcel.2004.08.009
- 48. Edmunds CE, Simpson LJ, Sale JE (2008) PCNA ubiquitination and REV1 define temporally distinct mechanisms for controlling translesion synthesis in the avian cell line DT40. Mol Cell 30: 519–529. doi: 10.1016/j.molcel.2008.03.024
- 49. Zietlow L, Smith LA, Bessho M, Bessho T (2009) Evidence for the involvement of human DNA polymerase N in the repair of DNA interstrand cross-links. Biochemistry 48: 11817–11824. doi: 10.1021/bi9015346
- 50. Bienko M, Green CM, Sabbioneda S, Crosetto N, Matic I, et al. (2010) Regulation of translesion synthesis DNA polymerase eta by monoubiquitination. Mol Cell 37: 396–407. doi: 10.1016/j.molcel.2009.12.039
- 51. Cui X, Brenneman M, Meyne J, Oshimura M, Goodwin EH, et al. (1999) The XRCC2 and XRCC3 repair genes are required for chromosome stability in mammalian cells. Mutat Res 434: 75–88. doi: 10.1016/s0921-8777(99)00010-5
- 52. Howlett NG, Taniguchi T, Olson S, Cox B, Waisfisz Q, et al. (2002) Biallelic inactivation of BRCA2 in Fanconi anemia. Science 297: 606–609. doi: 10.1126/science.1073834
- 53. Litman R, Peng M, Jin Z, Zhang F, Zhang J, et al. (2005) BACH1 is critical for homologous recombination and appears to be the Fanconi anemia gene product FANCJ. Cancer Cell 8: 255–265. doi: 10.1016/j.ccr.2005.08.004
- 54. Wu HI, Brown JA, Dorie MJ, Lazzeroni L, Brown JM (2004) Genome-wide identification of genes conferring resistance to the anticancer agents cisplatin, oxaliplatin, and mitomycin C. Cancer Res 64: 3940–3948. doi: 10.1158/0008-5472.can-03-3113
- 55. Uanschou C, Siwiec T, Pedrosa-Harand A, Kerzendorfer C, Sanchez-Moran E, et al. (2007) A novel plant gene essential for meiosis is related to the human CtIP and the yeast COM1/SAE2 gene. EMBO J 26: 5061–5070. doi: 10.1038/sj.emboj.7601913
- 56. Yu X, Chen J (2004) DNA damage-induced cell cycle checkpoint control requires CtIP, a phosphorylation-dependent binding partner of BRCA1 C-terminal domains. Mol Cell Biol 24: 9478–9486. doi: 10.1128/mcb.24.21.9478-9486.2004
- 57. Liu F, Lee WH (2006) CtIP activates its own and cyclin D1 promoters via the E2F/RB pathway during G1/S progression. Mol Cell Biol 26: 3124–3134. doi: 10.1128/mcb.26.8.3124-3134.2006
- 58. Limbo O, Chahwan C, Yamada Y, de Bruin RA, Wittenberg C, et al. (2007) Ctp1 is a cell-cycle-regulated protein that functions with Mre11 complex to control double-strand break repair by homologous recombination. Mol Cell 28: 134–146. doi: 10.1016/j.molcel.2007.09.009
- 59. Sartori AA, Lukas C, Coates J, Mistrik M, Fu S, et al. (2007) Human CtIP promotes DNA end resection. Nature 450: 509–514. doi: 10.1038/nature06337
- 60. Chen L, Nievera CJ, Lee AY, Wu X (2008) Cell cycle-dependent complex formation of BRCA1.CtIP.MRN is important for DNA double-strand break repair. J Biol Chem 283: 7713–7720. doi: 10.1074/jbc.m710245200
- 61. Williams RS, Dodson GE, Limbo O, Yamada Y, Williams JS, et al. (2009) Nbs1 flexibly tethers Ctp1 and Mre11-Rad50 to coordinate DNA double-strand break processing and repair. Cell 139: 87–99. doi: 10.1016/j.cell.2009.07.033
- 62. You Z, Shi LZ, Zhu Q, Wu P, Zhang YW, et al. (2009) CtIP links DNA double-strand break sensing to resection. Mol Cell 36: 954–969. doi: 10.1016/j.molcel.2009.12.002
- 63. Huertas P, Jackson SP (2009) Human CtIP mediates cell cycle control of DNA end resection and double strand break repair. J Biol Chem 284: 9558–9565. doi: 10.1074/jbc.m808906200
- 64. Hearst JE (1981) Psoralen photochemistry and nucleic acid structure. J Invest Dermatol 77: 39–44. doi: 10.1111/1523-1747.ep12479229
- 65. Kanne D, Straub K, Rapoport H, Hearst JE (1982) Psoralen-deoxyribonucleic acid photoreaction. Characterization of the monoaddition products from 8-methoxypsoralen and 4,5′8-trimethylpsoralen. Biochemistry 21: 861–871. doi: 10.1021/bi00534a008
- 66. Cleaver JE, Gruenert DC (1984) Repair of psoralen adducts in human DNA: differences among xeroderma pigmentosum complementation groups. J Invest Dermatol 82: 311–315. doi: 10.1111/1523-1747.ep12260596
- 67. Yan Z, Delannoy M, Ling C, Daee D, Osman F, et al. (2010) A histone-fold complex and FANCM form a conserved DNA-remodeling complex to maintain genome stability. Mol Cell 37: 865–878. doi: 10.1016/j.molcel.2010.01.039
- 68. Kong X, Mohanty SK, Stephens J, Heale JT, Gomez-Godinez V, et al. (2009) Comparative analysis of different laser systems to study cellular responses to DNA damage in mammalian cells. Nucleic Acids Res 37: e68. doi: 10.1093/nar/gkp221
- 69. Bostock CJ, Prescott DM, Kirkpatrick JB (1971) An evaluation of the double thymidine block for synchronizing mammalian cells at the G1-S border. Exp Cell Res 68: 163–168. doi: 10.1016/0014-4827(71)90599-4
- 70. Chen PL, Liu F, Cai S, Lin X, Li A, et al. (2005) Inactivation of CtIP leads to early embryonic lethality mediated by G1 restraint and to tumorigenesis by haploid insufficiency. Mol Cell Biol 25: 3535–3542. doi: 10.1128/mcb.25.9.3535-3542.2005
- 71. Fisher LA, Bessho M, Bessho T (2008) Processing of a psoralen DNA interstrand cross-link by XPF-ERCC1 complex in vitro. J Biol Chem 283: 1275–1281. doi: 10.1074/jbc.m708072200
- 72. Bakkenist CJ, Kastan MB (2003) DNA damage activates ATM through intermolecular autophosphorylation and dimer dissociation. Nature 421: 499–506. doi: 10.1038/nature01368
- 73. Lee JH, Paull TT (2007) Activation and regulation of ATM kinase activity in response to DNA double-strand breaks. Oncogene 26: 7741–7748. doi: 10.1038/sj.onc.1210872
- 74. Rogakou EP, Pilch DR, Orr AH, Ivanova VS, Bonner WM (1998) DNA double-stranded breaks induce histone H2AX phosphorylation on serine 139. J Biol Chem 273: 5858–5868. doi: 10.1074/jbc.273.10.5858
- 75. Ward IM, Chen J (2001) Histone H2AX is phosphorylated in an ATR-dependent manner in response to replicational stress. J Biol Chem 276: 47759–47762.
- 76. Ward IM, Minn K, Chen J (2004) UV-induced ataxia-telangiectasia-mutated and Rad3-related (ATR) activation requires replication stress. J Biol Chem 279: 9677–9680. doi: 10.1074/jbc.c300554200
- 77. Stiff T, Walker SA, Cerosaletti K, Goodarzi AA, Petermann E, et al. (2006) ATR-dependent phosphorylation and activation of ATM in response to UV treatment or replication fork stalling. EMBO J 25: 5775–5782. doi: 10.1038/sj.emboj.7601446
- 78. Huertas P, Cortes-Ledesma F, Sartori AA, Aguilera A, Jackson SP (2008) CDK targets Sae2 to control DNA-end resection and homologous recombination. Nature 455: 689–692. doi: 10.1038/nature07215
- 79. Yu X, Wu LC, Bowcock AM, Aronheim A, Baer R (1998) The C-terminal (BRCT) domains of BRCA1 interact in vivo with CtIP, a protein implicated in the CtBP pathway of transcriptional repression. J Biol Chem 273: 25388–25392. doi: 10.1074/jbc.273.39.25388
- 80. Yu X, Fu S, Lai M, Baer R, Chen J (2006) BRCA1 ubiquitinates its phosphorylation-dependent binding partner CtIP. Genes Dev 20: 1721–1726. doi: 10.1101/gad.1431006
- 81. Bruun D, Folias A, Akkari Y, Cox Y, Olson S, et al. (2003) siRNA depletion of BRCA1, but not BRCA2, causes increased genome instability in Fanconi anemia cells. DNA Repair (Amst) 2: 1007–1013. doi: 10.1016/s1568-7864(03)00112-5
- 82. Xiong J, Fan S, Meng Q, Schramm L, Wang C, et al. (2003) BRCA1 inhibition of telomerase activity in cultured cells. Mol Cell Biol 23: 8668–8690. doi: 10.1128/mcb.23.23.8668-8690.2003
- 83. Collis SJ, Ciccia A, Deans AJ, Horejsi Z, Martin JS, et al. (2008) FANCM and FAAP24 function in ATR-mediated checkpoint signaling independently of the Fanconi anemia core complex. Mol Cell 32: 313–324. doi: 10.1016/j.molcel.2008.10.014
- 84. Xue Y, Li Y, Guo R, Ling C, Wang W (2008) FANCM of the Fanconi anemia core complex is required for both monoubiquitination and DNA repair. Hum Mol Genet 17: 1641–1652. doi: 10.1093/hmg/ddn054
- 85. Bakker ST, van de Vrugt HJ, Rooimans MA, Oostra AB, Steltenpool J, et al. (2009) Fancm-deficient mice reveal unique features of Fanconi anemia complementation group M. Hum Mol Genet 18: 3484–3495. doi: 10.1093/hmg/ddp297
- 86. Botvinick EL, Berns MW (2005) Internet-based robotic laser scissors and tweezers microscopy. Microsc Res Tech 68: 65–74. doi: 10.1002/jemt.20216
- 87. Oh DH, Stanley RJ, Lin M, Hoeffler WK, Boxer SG, et al. (1997) Two-photon excitation of 4′-hydroxymethyl-4,5′,8-trimethylpsoralen. Photochem Photobiol 65: 91–95. doi: 10.1111/j.1751-1097.1997.tb01882.x
- 88. Viana NB, Rocha MS, Mesquita ON, Mazolli A, Neto PAM (2006) Characterization of objective transmittance for optical tweezers. Applied Optics 45: 4263–4269. doi: 10.1364/ao.45.004263
- 89. Mirzoeva OK, Petrini JH (2003) DNA replication-dependent nuclear dynamics of the Mre11 complex. Mol Cancer Res 1: 207–218.
- 90. Yu X, Baer R (2000) Nuclear localization and cell cycle-specific expression of CtIP, a protein that associates with the BRCA1 tumor suppressor. J Biol Chem 275: 18541–18549. doi: 10.1074/jbc.m909494199
- 91. Wang H, Shao Z, Shi LZ, Hwang PY, Truong LN, et al. (2012) CtIP Protein Dimerization Is Critical for Its Recruitment to Chromosomal DNA Double-stranded Breaks. J Biol Chem 287: 21471–21480. doi: 10.1074/jbc.m112.355354