Specificity of end resection pathways for double-strand break regions containing ribonucleotides and base lesions

ABSTRACT DNA double-strand break repair by homologous recombination begins with nucleolytic resection of the 5’ DNA strand at the break ends. Long-range resection is catalyzed by EXO1 and

BLM-DNA2, which likely have to navigate through ribonucleotides and damaged bases. Here, we show that a short stretch of ribonucleotides at the 5’ terminus stimulates resection by EXO1.

Ribonucleotides within a 5’ flap are resistant to cleavage by DNA2, and extended RNA:DNA hybrids inhibit both strand separation by BLM and resection by EXO1. Moreover, 8-oxo-guanine impedes

EXO1 but enhances resection by BLM-DNA2, and an apurinic/apyrimidinic site stimulates resection by BLM-DNA2 and DNA strand unwinding by BLM. Accordingly, depletion of OGG1 or APE1 leads to

greater dependence of DNA resection on DNA2. Importantly, RNase H2A deficiency impairs resection overall, which we attribute to the accumulation of long RNA:DNA hybrids at DNA ends. Our

results help explain why eukaryotic cells possess multiple resection nucleases. SIMILAR CONTENT BEING VIEWED BY OTHERS DNA END RESECTION AND ITS ROLE IN DNA REPLICATION AND DSB REPAIR CHOICE

IN MAMMALIAN CELLS Article Open access 30 October 2020 HLTF DISRUPTS CAS9-DNA POST-CLEAVAGE COMPLEXES TO ALLOW DNA BREAK PROCESSING Article Open access 10 July 2024 STRUCTURAL SNAPSHOTS OF

HUMAN DNA POLYMERASE Μ ENGAGED ON A DNA DOUBLE-STRAND BREAK Article Open access 22 September 2020 INTRODUCTION DNA double-strand breaks (DSBs) arise programmatically during meiosis, V(D)J

recombination, and immunoglobulin class switching and serve important functions therein1,2,3,4. DSBs are also induced by reactive metabolites, myriad chemotherapeutic agents, and upon

exposure of cells to radiation and mutagenic chemicals5,6. The persistence or mis-repair of DSBs can result in cell death or chromosomal rearrangements characteristic of cancer cells7. DSBs

are eliminated mainly via nonhomologous end joining (NHEJ) and homologous recombination (HR). In NHEJ, the break ends are processed and ligated, whereas homologous recombination (HR) entails

the engagement of the sister chromatid to template repair8,9,10. NHEJ is the predominant pathway in the G1 phase of the cell cycle, whereas HR becomes fully functional in the S and G2

phases when the sister chromatid becomes available. The decision to repair a DSB by NHEJ or HR is made at the onset of DNA end resection, a process in which nucleases degrade the

5′-terminated strands of the DSB, and that is influenced by a variety of factors including the cell cycle stage and lesion context11. The 3′ ssDNA tails stemming from resection serve as the

template for assembling the HR machinery harboring the recombinase RAD51, which searches for and invades the homologous region in the sister chromatid to form a displacement loop (D-loop),

followed by DNA synthesis, resolution of recombination intermediates, and ligation to complete repair8,9. Occasionally, the resected DNA ends can also undergo alternative end joining

(alt-EJ), in which break repair is guided by annealing of short homologous regions in separate 3′ DNA tails12,13. As such, alt-EJ invariably generates deletions and is therefore highly

mutagenic, and this often characterizes DNA breakpoints in cancer-associated chromosome translocations14. Thus, the choice of DSB repair pathway can have a strong impact on the maintenance

of genome integrity. Several conserved nucleases participate in the DNA end resection process. The MRE11-RAD50-NBS1 (MRN) complex, containing the MRE11 nuclease, works with CtIP to initiate

end resection by introducing a nick in the 5′ strand adjacent to DNA ends occluded by the NHEJ factor Ku15,16,17,18. MRN-CtIP can, subsequently, create a DNA gap via the 3′ to 5′ exonuclease

activity of MRE1119,20. Long-range 5′ strand resection initiated from the DNA nick or gap generated by MRN-CtIP is catalyzed either by the 5′ to 3′ exonuclease EXO1 or the endonuclease DNA2

in conjunction with the BLM helicase21,22,23,24. In the latter case, BLM separates DNA strands to generate a 5′ DNA flap for cleavage by DNA225,26,27. The selection pressure that has driven

eukaryotes to maintain seemingly redundant resection pathways has remained an enigma. In this study, we begin to address this issue by investigating the nucleolytic processing of DSB ends

with associated non-canonical nucleotides. The most common aberrant bases are ribonucleotides inserted by DNA polymerases or that stem from the deamination of cytosine residues to uracil28.

RNA segments of 8–12 nt can stem from incomplete removal of RNA primers during lagging strand DNA synthesis29,30,31. R-loop structures, which frequently arise during transcription, harbor

RNA:DNA hybrids ranging in size from less than 100 bp up to 2 kb32,33. Moreover, de novo RNA polymerase II-mediated transcription has been shown to create RNA:DNA hybrids at DSB

sites34,35,36. Reactive oxygen species generated during cellular metabolism induce lesions such as 8-oxo-guanine37. Furthermore, the processing of uracil, 8-oxo-G, and other damaged bases

leads to the formation of apurinic/apyrimidinic (AP) sites38. As such, the DNA end resection machinery is expected to encounter ribonucleotides and different DNA lesions. In this study, we

show that lesion context differentially influences the action and efficiency of the long-range resection machineries. Biological experiments yield evidence for a capability of the BLM-DNA2

ensemble to negotiate past these DNA lesions, and they also attest to the pivotal role of RNase H2 in the clearance of RNA–DNA hybrids during resection. These findings provide insights into

pathway crosstalk in DSB repair and help explain why eukaryotes engage multiple nucleases in DNA end resection. RESULTS STIMULATION OF EXO1 BY RNA RNA:DNA hybrids can arise at DSB sites

under different circumstances. Collision of a replication fork with a DNA lesion may lead to the formation of a DSB with 5′ terminal RNA that is a remnant of the RNA primer from lagging

strand DNA synthesis. Additionally, recent studies have shown that DSB formation is accompanied by de novo transcription39,40,41, which is expected to give rise to a varying length of 5′

terminated RNA at the break termini. Moreover, the collapse of a replication fork stalled at an R-loop would result in a DSB with an adjacent RNA:DNA hybrid32,33. To ask how such RNA content

might affect end resection, we tested human EXO1 on 3′ labeled 30-mer dsDNA substrates containing 1, 4, or 10 nt of RNA at the 5′ end. Surprisingly, 1 or 4 nt of 5′ RNA led to an increase

in EXO1 activity (Fig. 1a, lanes 1-15). EXO1 was able to resect through 10 nt of RNA with about the same efficiency as the control dsDNA substrate (Fig. 1a, lanes 16–20). These data suggest

that short stretches of 5′ RNA stimulate EXO1. Importantly, we observed the same stimulatory effect of RNA placed at the 5′ terminus with yeast Exo1 (Supplementary Fig. 1a). To prevent

degradation of the complementary unlabeled strand, we also performed the assay on substrates containing a 4-nt 5′ DNA overhang, which inhibits EXO1 activity. In this case, EXO1 was similarly

stimulated by a 4-nt RNA segment placed at the 5′ terminus of the susceptible strand (Supplementary Fig. 1b). The nuclease-deficient EXO1-D173A mutant42, purified in exactly the same manner

as the wild type counterpart, failed to cleave the substrate containing 4 nt of 5′ RNA (Fig. 1a, lanes 21–30), arguing against the possibility of an RNase contamination in our EXO1

preparations. A truncated version of human EXO1 containing the nuclease domain alone (residues 1–346), which was purified from _S. cerevisiae_, was also stimulated by 5′ RNA (Supplementary

Fig. 1c, lanes 1–10), as was a similar fragment (residues 1–352) purified from _E. coli_ (Supplementary Fig. 1c, lanes 11–20; gift from Lorena Beese). λ Exonuclease, which shares the 5′ to

3′ polarity of EXO1 but is structurally distinct, was blocked by RNA placed at either the 5′ terminus or at an internal location (Supplementary Fig. 1d). Together, these data show that the

ribonuclease activity we observed is intrinsic to EXO1 and that it is conserved in the yeast ortholog. DSB ends are rapidly occluded by the DNA end binding factor Ku in cells. Herein,

resection is initiated when the MRN-CtIP complex creates a nick adjacent to the Ku-bound DSB end. This nick serves as the entry site for EXO1 or BLM-DNA219. We therefore asked whether

stimulation of EXO1 by 5′ RNA also occurs at a nick. Again, strong stimulation of resection occurred when a 4-nt RNA segment was situated at the nick site (Fig. 1b). We also tested the

effect of RNA:DNA hybrid at DSBs containing a 3′ overhang, likely to be present at DSBs at a broken DNA replication fork. We note that a DNA substrate with a 5-nt 3′ overhang was acted on

with higher efficiency by EXO1 than an equivalent substrate without such an overhang (Fig. 1a, lanes 1–5, vs. Fig. 1c, lanes 1–5). Importantly, the addition of 1 or 4 nt of 5′ RNA at the

recessed end stimulated EXO1 activity (Fig. 1c, lanes 6–15). Unlike at a blunt end, however, stimulation was also observed upon extending the RNA to 10 nt (Fig. 1c, lanes 16–20). Given that

lagging strand RNA primers are typically 8–12 nt long43, these data suggest that EXO1 is more adept at resecting replication-associated DSB ends containing unprocessed remnants of Okazaki

fragments. To further investigate how the position of the RNA affects EXO1, we created a substrate in which an internal run of 4 ribonucleotides was placed 4 nt from the 5′ end (Fig. 1d).

Surprisingly, this internal RNA inhibited EXO1 and led to formation of a cleavage product corresponding to the location of the RNA (Fig. 1d). However, the RNA segment did not completely

block EXO1, as smaller products were still observed (Fig. 1d). We next radiolabeled the 5′ end of RNA-containing substrates to determine whether RNA stimulates resection initiation. The

results revealed that digestion of the first 5′ nucleotide of a 4-nt RNA-containing substrate occurs more efficiently (Fig. 2a, lanes 1–10), but that extending the RNA to create a full

RNA:DNA hybrid leads to inhibition (Fig. 2a, lanes 11–15). EXO1 showed no activity on dsRNA (Fig. 2a, lanes 16–20). Interestingly, EXO1 failed to digest the 5′ DNA end of a full DNA-RNA

hybrid (Fig. 2b, lanes 1–5). In fact, the presence of 15 nucleotides of RNA in the complementary strand led to near abrogation of DNA digestion (Fig. 2b, lanes 6–10). While a single

ribonucleotide had no discernible effect (Fig. 2b, lanes 11–15), slight inhibition was observed when the RNA length was increased to four nucleotides (Fig. 2b, lanes 16–20). Together, these

data show that even though the presence of a short 5′ RNA tract stimulates resection, RNA in the complementary strand restricts EXO1 activity on the 5′ DNA terminus. BYPASS OF RNA BY

BLM-DNA2 We also examined BLM-DNA2 for its ability to resect DNA substrates that harbor ribonucleotides. First, we tested 3′ end-labeled substrates containing 4 nt of RNA at the 5′ terminus

or at an internal location of the labeled strand. RNA in either location had little effect on resection efficiency by the BLM-DNA2-RPA ensemble, although a dramatic change in the cleavage

pattern was observed when RNA was present internally (Fig. 3a, lanes 6–10). Whereas DNA2 generated multiple cleavage products in the middle of the dsDNA substrate (Fig. 3a, lanes 1–5), it

incised primarily 1 nt after the embedded RNA to produce a 15-nt product (Fig. 3a, lanes 6–10). This suggests that DNA2 is unable to cleave within RNA but can act on neighboring DNA. We next

sought to determine the effects of RNA on BLM and DNA2 by testing the two enzymes on RNA-containing substrates separately. We first investigated how an RNA:DNA hybrid affects the BLM

helicase. A 4-nt tract of RNA at the 5′ end slightly stimulated BLM activity, whereas RNA placed at the internal locale attenuated unwinding (Fig. 3b). These inhibitory effects of RNA were

modest, however, and overall activity was comparable to that on dsDNA (Fig. 3b). BLM showed substantially reduced activity on a full RNA:DNA hybrid and was inactive toward dsRNA (Fig. 3c).

BLM translocates in the 3′ to 5′ direction while unwinding duplex DNA and shows the greatest activity on substrates with 3′ ssDNA overhangs44. We hypothesized that the reduction in BLM

activity on the RNA:DNA hybrid (Fig. 3c) might reflect an inability of the helicase to translocate on the RNA strand. To test this, we constructed a substrate with a 5-nt 3′ overhang on one

strand, which serves as an entry point for BLM to initiate translocation. Two versions were made in which the overhang-containing strand consisted of either RNA or DNA. While BLM efficiently

unwound the DNA substrate, it was barely active on the RNA:DNA hybrid (Fig. 3d). Together, these data show that BLM can negotiate through a short RNA patch while unwinding DNA, but becomes

strongly inhibited when the strand consists only of RNA, likely reflective of an inability of BLM to translocate on RNA. In agreement with this idea, the ATPase activity of BLM became

strongly attenuated when the ssDNA cofactor was replaced with ssRNA of the same sequence (Supplementary Fig. 2a). To test whether DNA2 is able to cleave within an embedded RNA tract, we

constructed Y-shaped substrates that mimic the intermediate generated as a result of strand separation by BLM. These substrates contain a 31-nt dsDNA region with 44-nt overhangs of either

DNA or with the 5′ DNA overhang harboring an internal patch of four ribonucleotides located 21 nt away from the duplex junction. Whereas DNA2 generated cleavage products throughout the 5′

DNA flap (Fig. 4a, lanes 1–7), it did not act on the embedded RNA as indicated by the lack of any product in the 52–56 nt range (Fig. 4a, lanes 8–14). Instead, a prominent product band of

~45 nt was seen (Fig. 4a, lanes 8–14), indicating that cleavage occurred in the DNA region downstream of the RNA. For clarity, an enlarged version of the relevant region of the gel from Fig.

 4a is shown in Supplementary Fig. 2b. A similar result was obtained in the presence of RPA (Fig. 4b) and with yeast Dna2 (Supplementary Fig. 2c). These data are consistent with our results

from examining BLM-DNA2-RPA (Fig. 3a) and indicate that DNA2 cannot incise within RNA. Previous studies have shown that RNA on the 5′ terminus of a flap stimulates yeast Dna2, but has no

effect on the _Pyroccocus horikoshii_ Dna2 ortholog45,46. We therefore tested whether a 4-nt segment of 5′ terminal RNA would affect flap cleavage by human DNA2. The human nuclease cleaved

the RNA-containing substrate with the same efficiency as the comparable DNA flap, regardless of the presence of RPA (Supplementary Fig. 2d). Thus, 5′ terminal RNA does not stimulate human

DNA2. DIFFERENTIAL EFFECTS OF 8-OXO-G AND AP SITE ON EXO1 AND DNA2 We next asked whether EXO1 could resect through two common base lesions, namely, 8-oxo-guanine, the most abundant oxidized

base in the human genome, and the AP site, created when a damaged base or uracil residue is removed by a lesion-specific DNA glycosylase or Uracil DNA Glycosylase, respectively. For this,

30-mer dsDNA substrates were created in which the lesion in question was situated at position 11 from the 5′ terminus. While the AP site had little or no effect on EXO1 (Fig. 5a, lanes

1–10), the 8-oxo-G residue caused the nuclease to stall about 4–5 nt upstream of the lesion (Fig. 5a, lanes 11–15). With higher EXO1 concentrations, we also observed a product corresponding

to stalling at the lesion site (Fig. 5a, lanes 14–15). These data suggest that 8-oxo-G residues that occur near DSB sites impede EXO1-dependent resection. Interestingly, the presence of an

AP site strongly stimulated resection by BLM-DNA2, while significant enhancement by the 8-oxo-G lesion was also seen (Fig. 5b). We hypothesized that disruption of base pairing by the AP site

might allow BLM to engage and unwind the substrate more readily. To test this idea, we constructed another substrate in which the AP site was replaced by adenine to create an A-C mismatch.

Consistent with the above premise, the DNA mismatch also enhanced DNA unwinding by BLM, albeit to a lesser degree when compared to the AP lesion (Fig. 5c, lanes 1–10, 16–20). In contrast,

8-oxo-G, which can base pair with the opposing cytosine but increases DNA bending47, had little or no effect on BLM-mediated DNA unwinding (Fig. 5c, lanes 11–15). Thus, in DSB end resection,

adjoining lesions that disrupt base pairing may facilitate DNA separation by BLM to create the requisite flap structure for DNA2 to act on. RESECTION THROUGH BASE LESIONS AND RNA:DNA

HYBRIDS IN CELLS To determine whether the differences in substrate specificity between EXO1 and BLM-DNA2 that we observed in vitro are relevant to resection in cells, we manipulated cellular

conditions to increase the burden of 8-oxo-G residues, AP sites, or RNA:DNA hybrids by performing siRNA knockdown against 8-oxo-G DNA Glycosylase (OGG1)48,49, Apurinic-Apyrimidinic

Endonuclease 1 (APE1)50,51, or RNase H2A32,33,52, respectively. We first irradiated U2OS cells following siRNA-mediated knockdown of EXO1 or DNA2 and assessed DNA end resection by

quantifying RPA foci53. Knockdown of only EXO1 or DNA2 resulted in significant impairment of resection (Supplementary Fig. 3a), in concordance with the established role of these nucleases in

long-range resection21,22,54. Next, we similarly tested cells with knockdown of OGG1 or APE1 along with additional depletion of either EXO1 or DNA2. Interestingly, radiation-induced RPA

foci numbers were higher in cells with OGG1 depletion, which might be due to increased DNA breakage as OGG1 loss has been shown to result in accumulation of single-strand breaks55.

Supplementary Fig. 3b; Fig. 6a). Importantly, additional depletion of EXO1 resulted in only a slight reduction in radiation-induced RPA foci, while DNA2 knockdown almost completely abrogated

resection (Fig. 6a). Similarly, in cells depleted for APE1 (Supplementary Fig. 3c), additional knockdown of EXO1 resulted in a small reduction in RPA foci, while knockdown of DNA2 led to a

more significant impairment of focus formation (Fig. 6b). These data suggest that DNA2 plays a more prominent role in the resection of DNA with an increased burden of 8-oxo-G residues or AP

sites. These findings are in congruence with our biochemical data showing that 8-oxo-G residues specifically impede EXO1 while upregulating resection efficiency by BLM-DNA2 (Figs. 5a, b),

and that AP sites stimulate unwinding by the DNA2-associated helicase BLM (Fig. 5c). Finally, we evaluated resection in cells with knockdown of RNase H2A, which is critical both for the

removal of interspersed ribonucleotides in DNA as well as for the degradation of the RNA component of R-loop structures32,33,52. Interestingly, radiation-induced RPA foci were significantly

reduced in cells with RNase H2A depletion, reflective of an overall impairment of resection (Supplementary Fig. 3d; Fig. 6c). Importantly, additional knockdown of EXO1 or DNA2 reduced RPA

foci modestly. Taken together, our results suggest that neither EXO1 nor BLM-DNA2 is able to efficiently resect through RNA–DNA hybrids that are targeted by RNase H2A. We note that these

data are in general concordance with our biochemical data showing that EXO1 and BLM-DNA2 are impeded by 5′ terminated RNA tracts with greater than ten ribonucleotides or a short RNA tract

present internally (Figs. 1d, 2a, 3c). DISCUSSION Multiple conserved DSB end resection pathways exist in eukaryotes from fungi to humans, but why such redundancy is necessary or desirable

has remained unclear. It has been proposed that these resection pathways might be suited for processing DNA breaks that harbor different lesions or are differentially engaged in various cell

cycle stages54. Here, we have documented properties of EXO1 and BLM-DNA2 at DSBs with physiologically relevant base lesions that help shed light on this issue. The principal findings of

this study, summarized in Fig. 6d, are (1) a short RNA tract located near the 5′ terminus enhances EXO1 activity, but an internal tract of RNA or a long RNA:DNA hybrid inhibits EXO1; (2) BLM

efficiently unwinds DNA containing a short stretch of RNA, but is impeded by a long RNA:DNA hybrid; (3) DNA2 cannot act on RNA located in a 5′ flap but can efficiently cleave an adjoining

DNA region; (4) EXO1 can digest an AP site but is impeded by 8-oxo-G; (5) an AP site stimulates BLM activity; (6) conditions that increase the load of 8-oxo-G residues or AP sites in cells

(i.e. loss of OGG1 or APE1) result in increased dependence on the DNA2-dependent resection pathway; and (7) loss of RNase H2A reduces resection efficiency in cells, likely due to the

accumulation of RNA:DNA hybrids that are inhibitory to both EXO1 and BLM-DNA2 at DSB sites. Altogether, our biochemical and cell-based analyses provide evidence that the apparently redundant

DNA end resection pathways are in fact adept for specific lesion contexts. Importantly, a short RNA tract stimulates EXO1, but inhibition occurs when the RNA length is increased (Fig. 1). A

long RNA:DNA hybrid tract causes the double helix to adopt the A form, which could explain the observed inhibitory effect on EXO1. We do not yet understand how the presence of a short 5′

RNA tract upregulates EXO1 activity. One possibility is that contacts between the enzyme and the downstream region of the substrate may confer such specificity42. The observation that

truncated EXO1 variants lacking the C-terminal domain are still stimulated by RNA (Supplementary Fig. 1c) suggests that protein–nucleic acid contacts crucial for this stimulatory effect are

retained in the N-terminal nuclease domain. While a short 5′ terminal RNA segment stimulates EXO1 (Fig. 1a-c), such an internal RNA tract causes EXO1 to pause (Fig. 1d). The mechanistic

basis of the inhibitory effect of internally situated RNA tracts remains to be delineated. The observation that 3′ RNA blocks EXO1 activity on the abutting 5′ DNA end (Fig. 2b) hints at a

mechanism for regulation of resection. Delaying resection might be desirable at DSBs undergoing ongoing transcription to maintain the integrity of the DNA template until transcription is

complete. Similarly, DSBs generated by R-loop cleavage might be left unresected until an alternate mechanism of resolution is engaged. We note that neither EXO1 nor BLM-DNA2 is adept at

resecting long RNA:DNA hybrids, which might be found at R-loop associated DSBs. In this case, the recruitment of an RNA:DNA helicase, such as SETX56, may lead to the clearance of such

RNA:DNA hybrids. We have demonstrated that, unlike EXO1, the BLM-DNA2 pathway bypasses regions of RNA to act on DNA downstream. This is consistent with a previous report showing that yeast

Dna2 can bypass a 12 nt 5′ RNA primer when cleaving Okazaki fragments45. The BLM helicase efficiently unwinds substrates with a short RNA:DNA hybrid (Fig. 3b) but is inactive on dsRNA (Fig. 

3c). That BLM is unable to unwind a substrate with a 3′ RNA overhang (Fig. 3d) suggests that BLM has minimal ability to translocate on RNA. We have shown biochemically that AP sites and

8-oxo-G residues, being among the most common base lesions in the genome57,58, exert differential effects on the two long-range resection pathways. While EXO1 is able to traverse through an

AP site, it is strongly impeded by 8-oxo-G (Fig. 5a). Interestingly, the AP site strongly stimulates end resection by BLM-DNA2 and DNA unwinding by BLM, while 8-oxo-G also exerts a

stimulatory effect on resection, albeit to a lesser degree compared to that seen with the AP site (Fig. 5b, c). Previous studies have shown that the AP site and 8-oxo-G lower the thermal

stability of DNA59,60. Our observation that a DNA mismatch also stimulates unwinding by BLM (Fig. 5c) suggests that this stimulation is likely mediated via transient unpairing of dsDNA to

create a 3′ flap from which BLM can initiate unwinding. Thus, our biochemical reconstitution studies suggest that duplex-destabilizing base lesions within the vicinity of a DSB are likely to

promote helicase-mediated resection. Predictions stemming from our biochemical analyses have been tested in the physiological setting by evaluation of DNA end resection in irradiated U2OS

cells with siRNA-mediated knockdown of OGG1, APE1, or RNase H2, in conjunction with knockdown of either EXO1 or DNA2. As expected from past studies in yeast and human cells21,22,54,61,62,63,

we have verified that resection of ionizing radiation (IR)-induced breaks is equally dependent upon EXO1 and DNA2 in U2OS cells (Supplementary Fig. 3a). However, upon knockdown of OGG1 in

these cells, resection becomes disproportionately dependent on DNA2 (Fig. 6a). This is consistent with our biochemical finding that 8-oxo-G specifically impedes EXO1 (Fig. 5a) while exerting

a stimulatory effect on the BLM-DNA2 resection pathway (Fig. 5b). Likewise, following the knockdown of APE1, which leads to the accumulation of AP sites in DNA, we have observed a greater

dependency on DNA2 relative to EXO1 for resection of IR-induced breaks (Fig. 6b). In congruence with these data, we have found stimulation of BLM-DNA2 by AP sites in vitro (Fig. 5b, c).

These results provide biological validation that the HR-specific DNA resection machinery is endowed with the wherewithal of removing certain DNA base lesions. RNase H2A plays an important

role in the clearance of RNA:DNA hybrids, such as those associated with R-loops64,65 or stemming from de novo transcription induced at DSB sites40,66. It also acts on ribonucleotides

embedded in DNA to initiate ribonucleotide excision repair67. Loss of RNase H2A is therefore expected to increase the RNA content in DNA. We found that extended RNA:DNA regions are

refractory to resection by both EXO1 and BLM-DNA2 in vitro (Figs. 2a and 3c), whereas individual and short stretches of ribonucleotides either stimulate EXO1 (if located at the 5′ end) (Fig.

 1a–c) or lead to pausing if located internally (Fig. 1d). Internal ribonucleotides can be efficiently resected by the BLM-DNA2 pathway, however, with DNA2 cleaving downstream within the

adjacent DNA (Fig. 4). Depletion of RNase H2A significantly impairs the resection of IR-induced breaks, and knockdown of either EXO1 or DNA2 has a modest effect on resection in RNase

H2A-depleted cells (Fig. 6c). We speculate that the impaired resection upon depletion of RNase H2A is primarily caused by the accumulation of R-loops or RNA:DNA hybrids stemming from de novo

transcription at DSBs64,65. It remains to be determined whether the involvement of RNase H2A in ribonucleotide excision repair67,68 is also germane for the regulation of DNA end resection.

Our findings are also relevant for studies on the repair of complex DSBs induced by accelerated ions of high linear-energy transfer (LET). Such ions are being increasingly used for cancer

therapy due to better dose distribution and greater DNA damage inflicted relative to low-LET X-rays69. Moreover, as components of galactic cosmic radiation, these ions also carry an

increased cancer risk relative to terrestrial radiation70,71. High-LET ions induce DSBs that are flanked by other types of base damage including oxidized bases and AP sites. These complex

DSBs are poorly repaired by NHEJ and are more reliant on the HR pathway for their resolution, which occurs only inefficiently72,73,74. A better understanding of how long-range nucleases

resect complex DSBs could lead to approaches to augment carbon ion therapy as well strategies to mitigate cancer risks from high-LET radiation. Altogether, our studies provide evidence for a

division of labor among resection nucleases that enables cells to efficiently process diverse lesions that arise endogenously and as a result of exposure to genotoxic agents. Moreover, they

furnish the conceptual and experimental framework to define the relationship between the HR machinery and other DNA repair pathways as well as R-loop avoidance and the nucleolytic

processing of complex DNA breaks. METHODS PROTEIN PURIFICATION Affinity epitope-tagged forms of EXO1, yExo1, DNA2, yDna2, BLM, and RPA were expressed and purified using our established

protocols24,26,27. DNA that codes for the EXO1(1-346) fragment was introduced into pESC-URA by gap repair and the protein was expressed and purified using the same procedure as the full

length protein (846 amino acid residues). EXO1 (1–352) was a gift from Lorena Beese and was purified from _E. coli_42. DNA SUBSTRATES The substrates were made by mixing a radiolabeled

oligonucleotide with a 2-fold excess of an unlabeled complementary oligonucleotide in TE buffer (20 mM Tris-HCl, 1 mM EDTA, pH 8.0) containing 50 mM NaCl and slow cooling from 95 °C to room

temperature over the course of 3 h. Substrates were separated from unannealed oligonucleotides in a native 10% acrylamide gel in TBE buffer (0.1 M Tris, 90 mM boric acid, 1 mM EDTA, pH 8.0)

at 4 °C, electroeluted from gel slices, and concentrated in an Amicon Ultracel 30K concentrator. DNA concentration was determined by UV absorbance. Oligonucleotide sequences are provided in

Supplementary Table 1. HELICASE AND NUCLEASE ASSAYS Helicase and nuclease assays were performed in buffer R (20 mM Na-HEPES, pH 7.5, 2 mM ATP, 0.1 mM DTT, 100 µg/ml BSA, 0.05% Triton-X 100,

2 mM MgCl2, and 100 mM KCl) and contained 2.5 nM DNA molecules. Reactions were conducted at 37 °C for the times indicated in the figure legends. After the addition of SDS to 0.2%, proteinase

K to 0.25 µg/µl, and 0.08% Orange G dye with a final glycerol concentration of 10%, the reaction mixtures were deproteinized for 5 min at 37 °C. Products were separated on acrylamide gels

in TBE buffer as indicated in the figure legends. For the analysis of endonucleolytic cleavage products generated by DNA2, reaction mixtures were processed in the same manner but were

fractionated under denaturing conditions with 7 M urea. Gels were dried onto Hybond membrane on top of Whatman filter paper (GE) and then analyzed in a BioRad Personal Molecular Imager FX

phosphorimager. Quantitation was by measuring loss of the substrate signal. ATPASE ASSAY ATPase assay was performed at 37 °C24. Briefly, BLM was incubated with an ssDNA or ssRNA 35-mer of

identical sequence (100 nM) in 10 μL of buffer [20 mM HEPES-KOH at pH 7.5, 5 mM Mg(C2H3O2)2, 1 mM DTT, 0.2 mM ATP, 0.4 μCi γ-32P-ATP] for the indicated time. The reaction was terminated by

adding 2 μL of the reaction to an equal volume of 0.5 M EDTA. Next, 1 μL of the reaction mixture was spotted onto a PEI cellulose TLC plate (Select Scientific), which was developed in with

0.15 M formic acid/0.15 M LiCl. The TLC plates were air-dried and then subjected to phosphorimaging analysis. CELL CULTURE AND IRRADIATION OF CELLS U2OS cells (obtained from the American

Type Culture Collection) were maintained in α-MEM medium, supplemented with 10% fetal bovine serum and penicillin/streptomycin in a humidified atmosphere with 5% CO2. Cells were irradiated

using the CellRad X-ray irradiator (Precision X-ray). TRANSFECTION OF CELLS Depletion of OGG1, APE1, RNase H2A, EXO1 or DNA2 was carried out by transfection with appropriate siRNAs

(Supplementary Table 2) using Lipofectamine RNAiMAX (Invitrogen). Cells were harvested 72 h later to verify knockdown by western blotting. Cells were transfected with scrambled siRNA as

control for all experiments. WESTERN BLOTTING AND ANTIBODIES Nuclear extracts for Western blotting were prepared by resuspending cell pellets in hypotonic lysis buffer (10 mM Tris-HCl pH

7.5, 1.5 mM MgCl2, 5 mM KCl, protease and phosphatase inhibitors), followed by nuclear extraction buffer (50 mM Tris-HCl pH 7.5, 0.5 M NaCl, 2 mM EDTA, 10% sucrose, 10% glycerol, protease

and phosphatase inhibitors). Whole cell extracts were prepared by resuspending cell pellets in 1xSDS protein lysis buffer (67.5 mM Tris pH 6.8, 25 mM NaCl, 0.5 mM EDTA, 12.5% Glycerol, 0.25%

SDS, DTT). The following primary antibodies were used: OGG1 (Abcam), APE1 (Santa Cruz Biotechnology), EXO1, RNase H2A (Bethyl), DNA2 (Thermo Fisher Scientific) and beta-actin (Cell

Signaling). The following secondary antibodies were used: horseradish peroxidase-conjugated secondary antibodies (Bio-Rad) and Alexa488/568-conjugated secondary antibodies (Invitrogen).

Antibody dilutions and catalogue numbers are provided in Supplementary Table 3. Uncropped gels are shown in Supplementary Figs. 4, 5. IMMUNOFLUORESCENCE STAINING Cells were seeded onto glass

chamber slides (Falcon) and immunostained with anti-RPA antibody 3 h after irradiation with 6 Gy. Cells were pre-extracted with buffer I (10 mM PIPES, pH 7.0, 100 mM NaCl, 300 mM Sucrose, 3

 mM MgCl2, 1 mM EGTA, 0.5% Triton X-100), extraction buffer II (10 mM Tris pH 7.5, 10 mM NaCl, 3 mM MgCl2, 1% Tween-40 and 0.5% sodium deoxycholate). Cells were fixed with 4%

paraformaldehyde/PBS and permeabilized with 0.5% Triton X-100 before incubation with antibodies. Images were captured using a Nikon Swept Field fluorescence microscope (×40 objective lens).

The average number of RPA foci per nucleus was determined after scoring at least 100 nuclei. Images were generated in the Core Optical Imaging Facility which is supported by UTHSCSA, NIH-NCI

P30 CA54174 (CTRC at UTHSCSA). Statistical analysis was carried out using GraphPad Prism software. REPORTING SUMMARY Further information on research design is available in the Nature

Research Reporting Summary linked to this article. DATA AVAILABILITY All data generated or analyzed during this study are included in this published article (and its supplementary

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Google Scholar  Download references ACKNOWLEDGEMENTS This study was supported by NIH grants R35 CA241801, R21 ES027154, RO1 CA197796, RO1 ES007061, RO1 CA205224, RO1 GM109645, PO1 CA092584,

and P30 CA054174, by the National Aeronautics and Space Administration Award NNX16AD78G, a Team Science Grant from the Gray Foundation under the Basser Initiative, and by CPRIT REI Award

RR180029. PS is the holder of the Robert A. Welch Distinguished Chair in Chemistry (AQ-0012). S.B. is the holder of the Mays Family Foundation Distinguished Chair in Oncology. AUTHOR

INFORMATION Author notes * Grace Hooks Present address: Department of Biochemistry, Duke University, Durham, NC, 27710, USA * Weibin Wang Present address: Department of Radiation Medicine,

School of Basic Medical Sciences, Peking University Health Science Center, Beijing, 100191, China * Adam S. Miller Present address: Regeneron, Rensselaer, NY, 12144, USA * Kevin A. Nguyen

Present address: David Geffen School of Medicine, University of California Los Angeles, Los Angeles, CA, 90095, USA AUTHORS AND AFFILIATIONS * Department of Molecular Biophysics and

Biochemistry, Yale University School of Medicine, New Haven, CT, 06510, USA James M. Daley, Grace Hooks, Weibin Wang, Adam S. Miller, Xiaoyu Xue, Kevin A. Nguyen & Patrick Sung *

Department of Biochemistry and Structural Biology, University of Texas Health Science Center, San Antonio, TX, 78229, USA James M. Daley, Hardeep Kaur, Sandeep Burma & Patrick Sung *

Department of Neurosurgery, University of Texas Health Science Center, San Antonio, TX, 78229, USA Nozomi Tomimatsu, Bipasha Mukherjee & Sandeep Burma * Department of Chemistry and

Biochemistry, Texas State University, San Marcos, TX, USA Xiaoyu Xue * Department of Medicine, University of Texas Health Science Center, San Antonio, TX, 78229, USA Elizabeth Williamson 

& Robert Hromas Authors * James M. Daley View author publications You can also search for this author inPubMed Google Scholar * Nozomi Tomimatsu View author publications You can also

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inPubMed Google Scholar * Sandeep Burma View author publications You can also search for this author inPubMed Google Scholar * Patrick Sung View author publications You can also search for

this author inPubMed Google Scholar CONTRIBUTIONS J.D., N.T., S.B., R.H., and P.S. conceived and designed experiments. J.D., N.T., and G.H. performed experiments. J.D., W.W., A.M., X.X.,

H.K., E.W., and K.N. generated expression constructs and purified proteins for the study. J.D., R.H., B.M., S.B., and P.S. analyzed the data and wrote the paper. CORRESPONDING AUTHORS

Correspondence to James M. Daley, Sandeep Burma or Patrick Sung. ETHICS DECLARATIONS COMPETING INTERESTS The authors declare no competing interests. ADDITIONAL INFORMATION PEER REVIEW

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permissions ABOUT THIS ARTICLE CITE THIS ARTICLE Daley, J.M., Tomimatsu, N., Hooks, G. _et al._ Specificity of end resection pathways for double-strand break regions containing

ribonucleotides and base lesions. _Nat Commun_ 11, 3088 (2020). https://doi.org/10.1038/s41467-020-16903-4 Download citation * Received: 24 July 2019 * Accepted: 29 May 2020 * Published: 18

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