CRISPR/Cas9-mediated homology-directed repair (HDR) is used for error-free targeted knock-in of foreign donor DNA. However, the low efficiency of HDR-mediated knock-in hinders establishment of knock-in clones. Double-strand breaks (DSBs) induced by CRISPR/Cas9 are preferentially repaired by non-homologous end joining (NHEJ) or microhomology-mediated end joining (MMEJ) before HDR can occur, thereby preventing HDR-mediated knock-in. NHEJ/MMEJ also cause random integrations, which give rise to false-positive knock-in events, or silently disrupt the genome. In this study, we optimized an HDR-mediated knock-in method for mouse embryonic stem cells (mESCs). We succeeded in improving efficiency of HDR-mediated knock-in of a plasmid donor while almost completely suppressing NHEJ/MMEJ-based integration by combining in vivo-linearization of the donor plasmid, transient knockdown of DNA polymerase θ, and chemical inhibition of DNA-dependent protein kinase (DNA-PK) by M3814. This method also dramatically improved the efficiency of biallelic knock-in; at the Rosa26a locus, 95% of HDR-mediated knock-in clones were biallelic. We designate this method BiPoD (Biallelic knock-in assisted by Pol θ and DNA-PK inhibition). BiPoD achieved simultaneous efficient biallelic knock-in into two loci. BiPoD, therefore, enables rapid and easy establishment of biallelic knock-in mESC lines.
Genomic integration of foreign donor DNA through homology-directed repair (HDR), exploited for classical gene-targeting technology, has been dramatically facilitated by development of the CRISPR/Cas9 system1. In this system, Cas9 endonuclease and single guide RNA (sgRNA) induce double-strand breaks (DSBs) at specific target sites into which donor DNA can be knocked-in. The broken sites are repaired by HDR using foreign donor DNA as a template, resulting in error-free targeted integration of the donor. HDR-mediated integration enables precise knock-in to be performed, including donor-based gene knock-out, tagging of endogenous genes, visualization of genomic regions, and insertion of expression cassettes into defined loci such as safe-harbor regions2.
Foreign donor DNA can be integrated into a host genome using any of several host DSB repair mechanisms. Therefore, to efficiently obtain HDR-mediated knock-in cells it is essential to reduce other types of integration events. Non-homologous end joining (NHEJ) is a major pathway for HDR-independent genomic integration, in which the ends of linearized donor DNA are directly ligated to the broken ends of genomic DNA3. This process is executed by multiple machineries, including DNA-dependent protein kinase (DNA-PK) and DNA ligase IV (LIG4)4,5. Another pathway is microhomology-mediated end joining (MMEJ). In contrast to NHEJ, the ends of donor and genomic DNA are aligned via microhomologous regions (≥ 1 bp) before joining6. Recent studies have shown that DNA polymerase theta (Pol θ or POLQ) plays a central role in MMEJ, thus this pathway is also called polymerase theta-mediated end joining7,8. Donor DNA is efficiently integrated into CRISPR/Cas9-induced DSB sites (on-target) through NHEJ or MMEJ with or without indel mutation9,10. Donor DNA can also be integrated into non-targeted sites (off-target) by way of NHEJ or MMEJ; this is called random integration11,12,13. Random integration is the easiest way to obtain transgenic cells, but the integration is unregulated resulting in unwanted genomic disruption and the generation of false-positive cells that incorporate marker genes at incorrect sites.
An advantage of HDR-mediated integration over NHEJ/MMEJ-based methods is the availability of negative selection markers, which are located outside the donor DNA homology arms and are only expressed if the entire donor is integrated through NHEJ/MMEJ. Frequently, however, only part of the donor is integrated into on- or off-target sites of the genome. In addition to donor DNA, part of the Cas9/sgRNA expression vector can also be integrated14. If negative selection markers are not integrated, it is very hard to detect the occurrence of such integrations. These "silent integrations'' disrupt the genome but are difficult to avoid through donor DNA design features. Because silent integrations occur by NHEJ and/or MMEJ, suppressing NHEJ/MMEJ events is of great importance to obtain scarless knock-in cells.
HDR is a rare event even when the CRISPR/Cas9 system is employed; therefore, it is difficult to obtain HDR-mediated knock-in cells15,16. The success rate for biallelic knock-in is extremely low, although it is required for various experimental strategies. Classically, two donor DNA templates with different marker genes [e.g., puromycin/blasticidin (BS) resistance genes and EGFP/mCherry] have been used to select biallelic knock-in cells17,18, but such dual markers are not always available. Furthermore, random integration of the antibiotic resistant genes can give rise to false-positive cells and prevent the acquisition of cells with precise biallelic knock-in. Thus, it would be advantageous to improve knock-in efficiency. In addition to HDR using foreign donor DNA as a template, DSBs induced by CRISPR/Cas9 are repaired by various other pathways, as described above. Once a site is repaired with accompanying genomic changes, such as indel mutations or donor insertions, the site is no longer a target of the same sgRNA/Cas9 complex. Therefore, HDR-mediated knock-in must occur before the target site is repaired by other mechanisms. Manipulating NHEJ and MMEJ pathways by chemical inhibitors, as well as overexpression and/or knockdown of pathway genes, have been tested in a large number of studies to improve HDR-mediated knock-in efficiency19,20,21. However, results from different studies have been inconsistent and a gold-standard method has not yet been established. Accordingly, biallelic knock-in of long donor DNA remains difficult and time-consuming.
Here, we show an optimized method for HDR-mediated knock-in applicable to mouse embryonic stem cells (mESCs). Combining in vivo-linearization of donor DNA, knockdown of the Polq gene, and chemical inhibition of DNA-PK, we achieved specific HDR-mediated knock-in with very high efficiency of biallelic integration. Our method, termed BiPoD (Biallelic knock-in assisted by Pol θ and DNA-PK inhibition), provides an easy and rapid way to obtain precise knock-in mESCs.
In vivo-linearization of a plasmid donor improves the efficiency of HDR-mediated knock-in
To evaluate the efficiency of HDR-mediated knock-in, Rosa26a, a widely used safe harbor locus in the mouse genome, was adopted as a target. The donor is shown in Fig. 1a. The CAG promoter-driven mCherry gene was inserted between 5′ and 3′ homology arms (0.8 kb and 0.9 kb, respectively), while an EGFP expression cassette was located downstream of the 3′ arm. If the donor is precisely integrated through HDR, the cells exhibit only red fluorescence (mCherry-positive/EGFP-negative, R+G−). The cells exhibit both red and green fluorescence if the entire donor sequence is integrated through a mechanism other than HDR, irrespective of integration site (mCherry-positive/EGFP-positive, R+G+). Another possibility is "partial integration", in which only part of the donor sequence is integrated into either Rosa26a or random loci. The fluorescence pattern depends on the region of the donor that is integrated. Cells are R+G+ if a majority of the donor is integrated, including both mCherry and EGFP expression cassettes, while integration of donor sequence fragments leads to R+G−, R−G+, or even R−G− cells, depending on which fragments are integrated. Here, we have to pay attention to partial integration. R+G− derived from partial integration could not be distinguished from that derived from legitimate HDR. Additionally, integration could not be detected if neither the mCherry nor EGFP expression cassette was included. We hypothesized that the occurrence of partial integration can be roughly estimated from the rate of R−G+ (only the EGFP expression cassette is integrated) because all partial integration events are thought to be caused by common mechanisms.
First, we compared the knock-in efficiency of in vivo- and in vitro-linearized plasmid donor DNA. To this end, a KpnI site and sgRosa26-1 sequence (a previously validated CRISPR/Cas9 target22) were located upstream of the 5′ arm (Fig. 1a). mESCs were transfected with the same amount of circular or KpnI-digested donor DNA. The circular donor is digested by Cas9 in the transfectants (in vivo-linearized), while the donor pre-digested by KpnI (in vitro-linearized) is directly used as an HDR template or integrated through other mechanisms. After simultaneous transfection of the donors with the expression vector of Cas9 and the sgRNA against Rosa26a, mESCs were cultured for 9 days to completely screen out transient expression of mCherry and/or EGFP and were then analyzed by flow cytometry (Fig. 1b,c). Only 2.5% of the in vitro-linearized donor transfectants became R+G−. However, the percentage of R−G+ transfectants was 2.4%, indicating that some or most of the R+G− cells occurred by partial integration and that the true occurrence of HDR-mediated knock-in was much lower than 2.5%. The percentage of R+G− cells was much higher when the in vivo-linearized donor was used (10%, p = 1.5 × 10–4 vs in vitro-linearization), while that of R−G+ cells was only 1.4%. These results indicated that the in vivo-linearization of the donor significantly increased the occurrence of HDR-mediated knock-in, although partial integration still occurred at a non-negligible level. In addition, the percentage of R+G+ cells resulting from non-HDR integration, was also increased when using the in vivo-linearized donor (1.1% to 8.9%, p = 5.0 × 10–4).
Combination of transient Polq knockdown with inhibition of DNA-PK decreases undesired integration of donors
To take advantage of the efficient HDR resulting from in vivo-linearization, we attempted to suppress non-HDR integration events during knock-in using in vivo-linearized donor. Random integration never occurs in POLQ and LIG4 double knock-out cells12,13. Pharmacological inhibition of DNA-PK by NU7441 in Polq KO mESCs increased the ratio of HDR to random integration to 1:1 at best13. Irreversible knock-out is not suitable for general knock-in experiments; therefore, we examined whether transient inhibition of Pol θ and DNA-PK in combination with in vivo-linearization of donor suppressed non-HDR integration events.
A number of small compounds that specifically and potently inhibit DNA-PK are available, whereas few specific Pol θ inhibitors have been reported. We, therefore, transiently knocked down Pol θ using shRNA. A series of experiments was performed as shown in Fig. 2a. To take into account the time required for repression by shRNA, mESCs were transfected with plasmids expressing shRNA against Polq or control shRNA and a puromycin-resistance gene 1 day before they were transfected with the circular plasmid donor targeting Rosa26a and the Cas9/sgRNA expression vector. These cells were treated with puromycin to select Polq-knockdown cells (Fig. 2b). The cells were also treated with a DNA-PK inhibitor for 3 days after transfection of the donor and Cas9/sgRNA vectors. After culture for 6 days (10 days from 1st transfection), the cells were analyzed by flow cytometry.
Initially, we examined the effect of NU7441 in combination with in vivo-linearization of donor DNA and transient knockdown of Polq (Fig. 2c). NU7441 was added to mESCs at 0 (DMSO only), 5, or 10 µM, because NU7441 is moderately toxic and no mESCs survived with 20 µM NU7441. Knockdown of Polq alone did not significantly change the occurrence of R+G− (mainly HDR) or R+G+ and R−G+ (non-HDR) cells. Polq knockdown + 10 µM NU7441 decreased the proportion of R+G+ and R−G+ cells from 16 to 4.5% (3.5-fold, p = 0.011), and the R+G+ and R−G+/R+G− ratio from 1.47 to 0.37 (p = 7.2 × 10–5). These results show that simultaneous transient inhibition of Pol θ by shRNA and DNA-PK by NU7441 is able to suppress non-HDR donor integration to some extent.
M3814 is a novel DNA-PK inhibitor, which can enhance HDR efficiency23,24. M3814 inhibits NHEJ more strongly than NU7441 in human induced pluripotent stem cells25 but there are no reports of using M3814 in combination with Pol θ inhibition. We examined the efficacy of M3148 instead of NU7441 in our scheme (Fig. 2d). We used M3814 at up to 10 µM because, similarly to NU7441, it exhibited moderate toxicity to mESCs. Transient treatment with 10 µM M3814 decreased the number of living cells, particularly in combination with Polq knockdown, but the surviving cells grew and formed dome-shaped colonies, a characteristic of undifferentiated mESCs (Fig. S1). Treatment with M3814 alone did not significantly affect the percentage of R+G+ and R−G+ cells (non-HDR integration). However, a combination of M3814 and Polq knockdown dramatically reduced the percentage of R+G+ and R−G+ cells. In particular, Polq knockdown + 10 µM M3814 decreased the percentage of R+G+ and R−G+ cells from 11 to 0.25% (43-fold, p = 4.5 × 10–5). Although the percentage of R+G− cells tended to drop non-significantly (7.1–4.4%), the R+G+ and R−G+/R+G− ratio was strikingly lower than that of control cells (1.57 vs 0.06, p = 3.9 × 10–4). These results indicate that in knock-in experiments using in vivo-linearized donor, and a combination of M3814 and Polq shRNA almost eliminates non-HDR integration events, without preventing HDR.
Knockdown of Polq alone markedly reduced the occurrence of R−G+ cells (1.8–0.47%, 3.9-fold, p = 3.8 × 10–4), although it did not significantly affect the occurrence of R+G+ cells (8.9–6.0%, 1.5-fold) (Fig. 2e). M3814 alone had no significant effect on the occurrence of R−G+ cells, even at 10 µM (Fig. 2e). Therefore, inhibition of Pol θ is essential for the decreased numbers of R−G+ cells, i.e., partial integration of donor DNA, and M3814 enhances the effect of Pol θ inhibition. These results indicated that the slight decrease in the percentage of R+G− cells by Polq knockdown with 5 or 10 µM M3814 (Fig. 2d) resulted from fewer false-positives caused by partial integrations.
Combination of Polq knockdown with M3814 treatment leads to biallelic knock-in
We focused on the fluorescence intensity of mCherry in the R+G− population (Fig. 3a and Fig. S2). The control cells (control shRNA + DMSO) showed a single fluorescence peak, while a second peak emerged in some conditions. There was an approximately two-fold difference between the intensity of these two peaks, indicating that the weaker peak and the stronger peak corresponded to cells harboring one and two copies of the mCherry gene, respectively. Given that the mCherry genes in the R+G− cells were mainly integrated through HDR, these two peaks were thought to be derived from monoallelic and biallelic integration of the mCherry gene into Rosa26a. The stronger peak was significantly increased by Polq shRNA + 10 µM NU7441, while the weaker peak was almost completely abolished by Polq shRNA + 10 µM M3814. These results indicate that simultaneous inhibition of Pol θ and DNA-PK improves biallelic knock-in efficiency. To confirm this speculation, clones isolated from the R+G− populations were analyzed by genomic PCR (Fig. 3b). The results indicated that only 6% of control cell clones (control shRNA + DMSO) harbored biallelic mCherry genes in the Rosa26a locus. However, 33% (8/24) and 95% (20/21) of clones were biallelic for Rosa26a mCherry in Polq shRNA + 10 µM NU7441 and Polq shRNA + 10 µM M3814 cells, respectively. These results were in good agreement with the fluorescence intensity patterns observed by flow cytometry analysis (Fig. 3a). Sanger sequencing of genomic PCR products confirmed that the donor DNA was precisely integrated into the Rosa26a locus in the Polq shRNA + 10 µM M3814 clones, demonstrating that this biallelic knock-in was mediated by HDR (Fig. 3c and Fig. S4). This method, using in vivo-linearized donor, Polq shRNA, and 10 µM M3814, was designated as BiPoD (Biallelic knock-in assisted by Pol θ and DNA-PK inhibition).
To understand the mechanism underlying efficient biallelic knock-in by BiPoD, the non-knock-in alleles generated under control shRNA + DMSO conditions were analyzed by Sanger sequencing. We discovered that all of the monoallelic clones had indel mutations in the CRISPR target sites (Fig. 3d and Fig. S5). These sites were no longer targets of CRISPR/Cas9 and subsequent HDR-mediated integration. It is likely that BiPoD prevents the formation of indel mutations by inhibiting NHEJ/MMEJ, thereby increasing the chance of HDR.
Influence of the combination of Polq knockdown and M3814 treatment on off-target cleavage
CRISPR/Cas9 editing occasionally exhibited off-target activity, resulting in cleavage of genomic loci with similar sequences to the target. Indel mutations frequently occurred when cleaved DNA was repaired by NHEJ or MMEJ. We examined whether BiPoD suppressed indel mutations caused by off-target activity. Candidate sites for off-target cleavage by the Rosa26a sgRNA were predicted using an off-target search tool (CRISTA)26. After transfection and culturing as described in Fig. 2a, R+G− (HDR-mediated knock-in) cells from control shRNA + DMSO or Polq shRNA + 10 µM M3814 conditions were collected and analyzed by amplicon sequencing (Fig. S6 and Supplementary Table 1). In the control shRNA + DMSO cell population, indel mutations were detected relatively frequently in one of the eight candidate sites but occurred infrequently in Polq shRNA + 10 µM M3814 cells at the same site. Although only a limited number of sites were examined, these results suggested that BiPoD had the potential to suppress indel mutations caused by off-target activity.
A combination of Polq knockdown and M3814 treatment can be used to tag endogenous genes
BiPoD was tested for its ability to tag the endogenous Sox2 gene, which encodes a nuclear-localized transcription factor that plays important roles in mESCs. A donor was designed to insert an EGFP-mAID tag at the C-terminal end of Sox2. Similar to the Rosa26a donor, a CRISPR target sequence was located upstream of the 5′ homology arm for in vivo-linearization. The BS-resistance gene (BSr) under control of the PGK promoter was integrated downstream of the EGFP-mAID tag sequence, and an mCherry expression cassette was located outside the 3′ homology arm to detect non-HDR integration events (Fig. 4a). If donor DNA integrated into the Sox2 locus through HDR, SOX2 would be expressed as a fusion protein with EGFP-mAID, which could then be confirmed by fluorescence microscopy or flow cytometry. mESCs were transfected with this donor together with a Cas9/sgRNA expression vector, and the transfectants were cultured until transient expression was lost. In the EGFP-positive (R−G+) cells, EGFP was mainly localized in the nucleus, which indicated that the SOX2-EGFP-mAID fusion protein was expressed (Fig. 4b). The EGFP-mAID tag is promoter-less; therefore, this donor is expected to express only mCherry (R+G−) when the whole donor sequence is non-HDR integrated, or in the case of partial integrations. A minor fraction of cells expressed both nuclear-localized EGFP and diffused mCherry (R+G+) (Fig. 4c). This likely resulted from incomplete HDR, simultaneous occurrence of both HDR- and non-HDR-mediated integrations, or fusion with other proteins because the homology arm included sequence encoding the nuclear localization signal of SOX227. In comparison to the control conditions, the percentage of R+G+ and R+G− cells (non-HDR) was drastically decreased by Polq shRNA + 10 µM M3814 (2.4–0.15%, p = 3.0 × 10–4) (Fig. 4d). Although the percentage of R−G+ cells was also decreased by Polq shRNA + 10 µM M3814 (7.8–2.8%, p = 0.0035), the R+G+ and R+G–/R–G+ ratio was significantly lower for Polq shRNA + 10 µM M3814 cells (0.31 vs 0.05, p = 2.6 × 10–4) (Fig. 4d,e). Additionally, the intensity of EGFP in the R−G+ population was significantly shifted from the weaker (monoallelic) to the stronger (biallelic) peak (Fig. 4f and Fig. S7). Taken together, BiPoD was able to tag endogenous genes.
Simultaneous biallelic knock-in into two different loci
Next, we attempted simultaneous knock-in of Rosa26a-mCherry and Sox2-EGFP-mAID (Fig. 5a). The donor DNA and Cas9/sgRNA expression vectors were the same as those used in the single knock-in experiments. Polq knockdown- or control-mESCs were simultaneously transfected with these four plasmids. To maintain the total amount of DNA transfected, the amounts of each DNA were half those used in the single knock-in experiments. Polq knockdown cells were treated with 10 µM M3814, while control cells (control shRNA) were treated with DMSO. Transfected cells were treated with BS after Day 8. Surviving cells were predicted to harbor the BSr gene from the Sox2 donor, regardless of the manner of integration. Isolated clones from surviving cells were expanded and analyzed by fluorescence microscopy and genomic PCR (Fig. 5b,c and Fig. S8). We confirmed that the larger PCR products were derived from HDR-mediated knock-in alleles using Sanger sequencing (Figs. S9 and S10). Only one control clone (control shRNA + DMSO) (5%, 1/20) harbored knock-in alleles of Rosa26a-mCherry and Sox2-EGFP-mAID, both of which were monoallelic. Despite BS-resistance, 65% (13/20) of control clones did not harbor a knock-in Sox2 allele. If the entire region of the Sox2 donor is integrated in a non-HDR manner, mCherry is expressed as the negative selection marker. However, control clones 4 and 19 did not exhibit red fluorescence, probably because only part of the Sox2 donor was integrated. In addition, PCR products of unexpected sizes were found in many control clones, indicating that large deletions or incorrect recombinations occurred in the target regions. In contrast, 96% (22/23) of Polq shRNA + 10 µM M3814 clones harbored a knock-in Sox2 allele. Interestingly, 39% (9/23) of these clones harbored both Rosa26a-mCherry and Sox2-EGFP-mAID, and 26% (6/23) were biallelic at both loci. In contrast to the control, the fluorescence patterns of each Polq shRNA + 10 µM M3814 clone were almost completely consistent with those expected from the knock-in patterns (mCherry from Rosa26a-mCherry and Nuc-EGFP from Sox2-EGFP-mAID), and no unexpected PCR products were observed. These results demonstrated that BiPoD enabled efficient biallelic knock-in into two different loci simultaneously.
Treatment with novobiocin and M3814 increases biallelic knock-in efficiency
Novobiocin, a small-molecule antibiotic, was recently reported as an inhibitor of Pol θ28. We examined whether novobiocin can improve the efficiency of HDR-mediated knock-in in our scheme (Fig. 6a). When used in combination with 10 µM M3814, treatment with 300 µM novobiocin for 3 days completely killed mESCs, while a fraction of mESCs survived with 200 µM novobiocin. Flow cytometry analyses showed that 200 µM novobiocin + 10 µM M3814 decreased the proportion of R+G+ and R+G− cells, but the effect was not statistically different from that of 10 µM M3814 alone (Fig. 6b). These results indicated that novobiocin exerted a weaker effect compared with shRNA-mediated knockdown of Polq. However, 200 µM novobiocin + 10 µM M3814 increased biallelic knock-in, whereas there was almost no change for cells treated with novobiocin or M3814 alone (Fig. 6c and Fig. S12). Although the effect was weaker than that of shRNA-mediated knockdown of Polq, novobiocin exhibited synergistic effects with M3814, at least on the increase of biallelic knock-in.
Here, we propose BiPoD, an HDR-mediated knock-in method comprising in vivo-linearization of donors, knockdown of Polq, and inhibition of DNA-PK by M3814. Compared with the classic knock-in method, BiPoD is an improvement on two points: an increased rate of HDR by in vivo-linearization, and a decreased rate of non-HDR integration by inhibition of Pol θ and DNA-PK (Fig. 7a). BiPoD is a simple and low-cost method: donor, expression of Cas9/sgRNA, and knockdown of Polq are all achieved by easily prepared plasmids. BiPoD enables easy and rapid establishment of biallelic knock-in mESCs.
Using the Rosa26a locus as a model, we show that in vivo-linearization of the donor increased the percentage of R+G− cells, mainly by HDR-mediated knock-in. CRISPR/Cas9 may cleave the genomic target site and donor DNA simultaneously, thereby synchronizing the supply and demand of homologous sequences and elevating HDR efficiency29,30. Recently, Yao et al. proposed a novel knock-in approach termed homology-mediated end joining (HMEJ), which uses a donor vector with long homology arms (~ 800 bp) with the CRISPR target site outside of each homology arm30. A similar method (termed GeneWeld) was established by Wierson et al., which uses shorter arms (24–48 bp) than HMEJ31. In these methods, both homology arms are liberated by a double cut, and the donor DNA is integrated into the target site through HDR, NHEJ, and/or MMEJ, which increases knock-in efficiency30,31. In contrast, we confirmed that a single CRISPR target site at the end of one homology arm was enough to significantly increase HDR-mediated knock-in, compared with donor linearization before transfection. NHEJ and MMEJ are inhibited in the BiPoD procedure, so the knock-in efficiency cannot be increased through NHEJ/MMEJ. Therefore, a double cut was not advantageous for BiPoD. An advantage of the single cut is that negative selection markers to detect unwanted integration via non-HDR pathways can be used. In vivo-linearization also increased the percentage of R+G+ cells, probably generated by integration of all or almost all regions of the donor. The design of the Rosa26a donor, in which the single CRISPR target sequence was located outside one of the homology arms, is similar to that used in a previous report9. They showed that the entire donor DNA sequence is efficiently integrated into the Cas9-induced DSB site when the donor had one CRISPR target sequence. Similarly, on-target integration of the entire donor DNA sequence probably increased the R+G+ population in our study. However, the R−G+ population was not increased by in vivo-linearization, indicating that the occurrence of random integrations was not substantially affected.
Recent studies have shown that simultaneous inhibition of Pol θ and NHEJ-related factors abolishes random integration through NHEJ and MMEJ12,13. These studies used constitutive knock-out of genes encoding Pol θ and subunits of LIG4. We demonstrated that transient knockdown of Polq by shRNA was also effective, making the strategy applicable for general knock-in experiments. Inhibition of Pol θ was important, particularly for suppressing partial integration of donor DNA. Another important advance concerns DNA-PK inhibitors. NU7441 failed to completely abolish non-HDR integrations in Polq knock-out or Polq knockdown mESCs (Ref.13 and Fig. 2c); however, this was achieved using M3814. The effect of M3814 alone on knock-in into both Rosa26a and Sox2 loci was not significant; however, the combination of M3814 and Polq knockdown almost completely abolished non-HDR integration events, without preventing HDR. Accordingly, large deletion and incorrect integration at the target loci, probably mediated by NHEJ and MMEJ, were completely suppressed by M3814 + Polq knockdown (Figs. 3b, 5b,c). Furthermore, as described above, M3814 + Polq knockdown suppressed indel mutations at off-target sites. When both NHEJ and MMEJ are inhibited, off-target cleavage may be repaired by a rare HDR using the sister chromatid as a template or not repaired resulting in apoptosis, either of which decreases the occurrence of cells harboring off-target indel mutations.
M3814 + Polq knockdown dramatically improved the efficiency of biallelic knock-in. In this study, 95% of R+G− cells (i.e. 4.2% of all cells) harbored biallelic mCherry genes in Rosa26a (Figs. 2d and 3b). This high efficiency of BiPoD enables biallelic knock-in cells to be obtained without the need for marker genes during clone isolation. Furthermore, BiPoD achieved simultaneous biallelic knock-in at two different loci. In this study, only one marker gene (BSr) was used for selection of stably integrated cells. Consequently, 26% of selected cells were double-biallelic. Thus, double-biallelic knock-in mESCs can be established easily and quickly by BiPoD using only one selectable marker. The increased biallelic knock-in efficiency is likely to result from inhibition of both NHEJ and MMEJ pathways. Generally, NHEJ/MMEJ repairs CRISPR/Cas9-induced DSB sites faster than HDR and causes indel mutations or insertion of donor. Such sites are no longer targeted by CRISPR/Cas9 and subsequent HDR. Indeed, the non-knock-in alleles had indel mutations at the CRISPR target sites in all of the monoallelic knock-in clones generated by the control conditions, indicating that these mutations prevented HDR-mediated knock-in. However, DSB sites have to be repaired by HDR using foreign donors or undamaged chromosomes as templates when both NHEJ/MMEJ are inactivated, although sites repaired using undamaged chromosomes recover their original genomic sequence and can, therefore, be cleaved by CRISPR/Cas9 again. Consequently, all target alleles are eventually cleaved and repaired by HDR using donor DNAs, resulting in biallelic knock-in or apoptosis.
During the knock-in experiments, several types of partial integration were observed. Knock-in into Rosa26a generated a minor population of cells that only expressed a negative selection marker (R−G+) (Fig. 2). Simultaneous knock-in into Rosa26a and Sox2 generated some clones that harbored randomly integrated Sox2 donors, but that did not express the negative expression marker (Fig. 5b). Such partial integrations create false-positives and prevent rapid acquisition of desired cell lines. These results also indicate that a similar amount of silent integration, which is undetectable by marker expression, occurs concomitantly and silently disrupts the genome. Knock-in into Rosa26a showed that in vivo-linearization did not increase the percentage of R−G+ cells, which decreased the chance of obtaining cells harboring partial integrations. Furthermore, functional inhibition of Pol θ significantly decreased partial integration, and Polq knockdown combined with M3814 treatment abolished almost all partial integrations. Therefore, BiPoD facilitates and accelerates successful acquisition of scarless knock-in cells by excluding partial integrations.
Why Polq knockdown decreases partial integration (R−G+) but not integration of all or almost all regions (R+G+) of the donor DNA in the Rosa26a knock-in experiments is an open question. The mechanism underlying integration of only the inner part of the donor DNA, i.e., exclusion of the outer regions, is also unclear. One possible hypothesis is that partial integration depends on long-range end resection of the donor DNA followed by MMEJ. MMEJ is initialized with 5′ to 3′ resection at the ends of DSBs to generate 3′ single-stranded tails, and then the exposed microhomologous sequences are annealed for the subsequent repair process32. Overexpression of exonuclease 1 (EXO1), one of the nucleases responsible for end resection, enhances efficiency of MMEJ-based knock-in, likely through resection of the DSB ends of both the endogenous locus and the donor vector33. Interestingly, EXO1 is able to resect 5′ strands greater than 3 kb in human cells34. Therefore, EXO1 is capable of deeply resecting the ends of linearized donor vectors to generate long 3′ single-stranded tails at both ends of the donor DNA. If the single-strand sequence located near the center of the donor DNA anneals to the genome through microhomology, the MMEJ machinery removes the region outside the microhomology as a single-strand flap, resulting in genomic integration of only the inner part of the donor vector (Fig. 7b). Thus, it is possible that inactivation of MMEJ by Polq knockdown suppresses partial integration. Recently, MMEJ, but not NHEJ, was suggested as a cause of large deletions at DSB sites induced by CRISPR/Cas9, likely through long-range resection of the DSB ends35. The mechanism underlying partial integration needs to be investigated in future studies. Non-resected full-length linearized donor DNA can be integrated through NHEJ. Therefore, it is plausible that Polq knockdown alone does not sufficiently block integration of all regions of the donor vector (R+G+).
BiPoD requires a two-step transfection protocol, followed by antibiotic-selection of Pol θ-downregulated cells, limiting the application of this method. Chemical inhibitors against Pol θ are a promising solution to this problem. Novobiocin is the only published small compound that inhibits Pol θ28. We found that novobiocin + M3814 improved biallelic knock-in efficiency compared with M3814 alone. However, the effects of novobiocin were clearly weaker than those of shRNA knockdown, even if used at the maximum sub-toxic concentration. This is likely to be because of the specificity of the activity of novobiocin. Novobiocin was used at 50–200 µM to suppress Pol θ activity in U2OS cells28; however, novobiocin weakly inhibits eukaryotic topoisomerase II and HSP9036,37. Partial inhibition of these extra target proteins might potentiate the cytotoxicity of novobiocin, preventing sufficient inactivation of Pol θ. Pol θ is a promising target for cancer therapy; therefore, Pol θ inhibitors are currently in development in multiple companies and laboratories38. More specific and potent Pol θ inhibitors will enable a one-step transfection BiPoD protocol that does not need antibiotic selection.
Materials and methods
NU7441 and M3814 were purchased from Cayman Chemical (Ann Arbor, MI). These reagents were dissolved in DMSO and used with a final DMSO concentration of 0.1%. Puromycin (FUJIFILM Wako Pure Chemical Corporation, Osaka, Japan) and Blasticidin (MP Biomedicals, Santa Ana, CA) were dissolved in sterilized water and used for selection at 1 µg/mL and 10 µg/mL, respectively. Novobiocin sodium (Kanto Chemical Co., Inc., Tokyo, Japan) was dissolved in sterilized water and used at the indicated concentrations.
pX330-U6-Chimeric_BB-CBh-hSpCas9 (a gift from Feng Zhang, Addgene #42230) was used for expression of Cas9/sgRNA. The CRISPR target sequences were as follows: Rosa26a, 5′-ACTCCAGTCTTTCTAGAAGA-3′22 and Sox2, 5′-CAGCCCTCACATGTGCGACA-3′39. The Rosa26a donor vector was based on pROSA26-PA (a gift from Frank Costantini, Addgene #21271). The mCherry expression cassette from pCAGGS-mCherry (a gift from Phil Sharp, Addgene #41583) was inserted between the homology arms. The guide RNA sequence targeting Rosa26a with a PAM sequence was inserted into the KpnI and HindIII sites, while the EGFP expression cassette was inserted into the SacI and NcoI sites. The Sox2 donor vector was constructed as follows: EGFP-mAID and the PGK-BSD expression cassette were flanked by the homology arms for Sox2. The mAID-PGK-BSD sequence was derived from pMK391 (a gift from Masato Kanemaki, RIKEN BRC #RDB1681940). Silent mutations were introduced into the 5′ homology arm to prevent targeting by CRISPR/Cas9. A stretch of sequence was inserted upstream of the pCAGGS-mCherry CAG promoter. Detailed maps of the donor plasmids are shown in Figs. S13 and S14. The puromycin-selectable shRNA expression vector (a gift from Jun Ohgane) is the same as that described previously41: a pENTR-based shRNA expression vector (a gift from Makoto Miyagishi and Hideo Akashi) with a puromycin resistance gene expression cassette followed by an internal ribosome entry site (IRES) and Venus gene42.
The J1 mESC line was purchased from American Type Culture Collection. mESCs were cultured on 0.1% gelatin-coated dishes in KnockOut DMEM (Thermo Fisher Scientific, Waltham, MA) supplemented with 15% fetal bovine serum (Biowest, Nuaillé, France), 1000 U/mL leukemia inhibitory factor (Merck Millipore, Burlington, MA), 1% l-glutamine (FUJIFILM Wako Pure Chemical Corporation), 1% non-essential amino acids (FUJIFILM Wako Pure Chemical Corporation), 0.18% 2-mercaptoethanol (Thermo Fisher Scientific), and 1% penicillin–streptomycin (FUJIFILM Wako Pure Chemical Corporation). Leukemia inhibitory factor was added at 2000 U/mL during DNA-PK inhibitor treatment and simultaneous knock-in experiments.
Transfection was performed using Lipofectamine 2000 (Thermo Fisher Scientific) and the single suspension method43. Briefly, trypsinized mESCs were collected in a 1.5 mL tube. After removal of supernatant, cells were resuspended in DNA-Lipofectamine 2000 complex in Opti-MEM (Thermo Fisher Scientific) by pipetting, then incubated at room temperature for 5 min. The mESCs were then diluted in mESC medium (without penicillin–streptomycin) and transferred to a gelatin-coated plate for culture. When the transfectants were treated with DNA-PK and/or Pol θ inhibitors, the medium was replaced with fresh medium containing the inhibitors 4 h after transfection.
Fluorescence of living cells was analyzed using an SH800 Cell Sorter (Sony, Tokyo, Japan).
Knockdown of Polq
The shRNA target sequences were 5′-GAATATGAGTGATAGTATACT-3′ (Polq) and 5′-CAACAAGATGAAGAGCACCAA-3′ (scrambled, negative control). To confirm knockdown, the puromycin-selected transfectants were directly subjected to RT-qPCR analysis using the CellAmp™ Direct TB Green® RT-qPCR Kit (TaKaRa Bio Inc., Shiga, Japan) at 3 days after transfection. The primers for RT-qPCR were as follows: Polq, 5′-GACTCTGGGTTCCACCAGAAG-3′ and 5′-GGCCTGGTAAAGGATGCAAG-3′, Actb, 5′-TTCTACAATGAGCTGCGTGTGG-3′ and 5′-ATGGCTGGGGTGTTGAAGGT-3′.
Genotyping of Rosa26a knock-in clones
R+G− cells were collected by fluorescence activated cell sorting (FACS) using an SH800 Cell Sorter (Sony) and seeded on gelatin-coated dishes at low density to obtain clonal colonies. After culturing for 4 days, colonies were picked and transferred to a 96-well plate. During picking, we ensured that isolated colonies were not contaminated with other cells. On the following day, the cells were observed by fluorescence microscopy to confirm whether they were R+G−. R−G− clones found here were excluded from subsequent experiments. We also confirmed that there was no contamination of R−G−, R−G+, or R+G+ cells in the R+G− clones. The R+G− clones were expanded for 6–7 days. Their fluorescence was observed again just before genomic DNA extraction to confirm that all cells were R+G−. Then, cells were lysed in 0.1 M Tris–HCl buffer (pH 8.0) containing 0.2% sodium lauryl sulfate, 5 mM ethylenediaminetetraacetic acid-2Na, 200 mM NaCl, and 5 µg/mL Proteinase K (FUJIFILM Wako Pure Chemical Corporation). Genomic DNA for each clone was extracted by isopropanol precipitation followed by rinsing with 70% ethanol and dissolving in 0.1× Tris–EDTA buffer (Thermo Fisher Scientific). PCR was performed with KOD FX Neo (TOYOBO, Osaka, Japan) according to the manufacturer's instructions. The primers for amplification of the Rosa26a locus were 5′-CTCCGGCTCCTCAGAGAGCCTCGGCTAGGTAG-3′ (outside the right arm), 5′-GGAAAATACTCCGAGGCGGATCACAAGCAATAATAACCTGTAG-3′ (inside the left arm), and 5′-ACGTGTAGAATGCCATGAGTCAAGCCAGTCCAAGAG-3′ (outside the left arm). PCR products of knock-in alleles (amplified with outside primers) were purified using the Fast Gene Gel/PCR Extraction Kit (Nippon Genetics Co., Ltd., Tokyo, Japan) and sequenced by FASMAC Corp. (Kanagawa, Japan) using the Sanger method. Sequencing primers for Rosa26a knock-in allele were 5′-CACAAGACCTTAGGTCAGGAAAG-3′ (L), 5′-GGAAAATACTCCGAGGCGGATCACAAGCAATAATAACCTGTAG-3′ (In), and 5′-AGGGCGGCTTGGTGCGTTTG-3′ (R).
Genotyping of double knock-in clones
Cloning and analysis were performed as for Rosa26a knock-in clones with several modifications. The transfectants were treated with 10 µg/mL BS for 2 days, then passaged at low density. After culturing for 4 days with 10 µg/mL BS, colonies were picked into a 96-well plate, cultured for 5 days, passaged into a 48-well plate and further cultured for 2 days. Genomic DNA was then extracted. Fluorescence was observed at 3 days after colony picking and just before genomic DNA extraction to identify and exclude contaminated clones. The primers for amplification of the Sox2 locus were 5′-GAGAACCCCAAGATGCACAACTCGGAGATCAGCAAG-3′ (outside the left arm) and 5′-CATGGATTCTCGGCAGCCTGATTCCAATAACAGAG-3′ (outside the right arm). PCR products of knock-in alleles were purified and sequenced by FASMAC Corp. as described above. Sequencing primers for Sox2 knock-in allele were 5′- CTGCTCCTGCATCATGCTGTAG-3′ (L), 5′- AAGCACTGCACGCCGTAGGT-3′ (In), and 5′- GATTCCAATAACAGAGCCGAATC-3′ (R).
Living mESCs were observed with a fluorescence IX71 microscope (Olympus, Tokyo, Japan) at 20× magnification. Nuclei were stained with Hoechst 33342 (Dojindo Laboratories, Kumamoto, Japan).
A search for off-target candidate sites for Rosa26a sgRNA (5′-ACTCCAGTCTTTCTAGAAGA-3′) was conducted using the CRISPR Target Assessment (CRISTA) tool26. Excluding sites inside repeat sequences, eight target sites with the highest CRISTA scores were selected. R+G− cells generated in control shRNA + DMSO or Polq shRNA + 10 µM M3814 conditions were collected using FACS, cultured for 2–4 days, and genomic DNA was extracted. Genomic regions containing off-target candidate sites were amplified by PCR with PrimeSTAR HS high-fidelity DNA polymerase (TaKaRa Bio Inc.). After confirming specific amplification, the PCR products were analyzed by deep sequencing conducted by Bioengineering Lab. Co., Ltd. (Kanagawa, Japan). Occurrence rates of indel mutations were analyzed with CRISPResso244. Details of the off-target candidate sites, primer sequences, and amplicons are shown in Supplementary Table 2.
All experiments were repeated three times. Statistical significance was determined by Student's t-test (two samples) or Tukey’s multiple comparison test (all pairs from ≥ 3 samples) using R software. All P-values from Tukey’s multiple comparison tests are shown in Supplementary Tables 3–6.
The datasets generated during and/or analyzed during the current study are available from the corresponding author on reasonable request.
Mali, P. et al. RNA-guided human genome engineering via Cas9. Science 339, 823–826 (2013).
Banan, M. Recent advances in CRISPR/Cas9-mediated knock-ins in mammalian cells. J. Biotechnol. 308, 1–9 (2020).
Davis, A. J. & Chen, D. J. DNA double strand break repair via non-homologous end-joining. Transl. Cancer Res. 2, 130–143 (2013).
Lieber, M. R. The mechanism of DSB repair by the NHEJ. Annu. Rev. Biochem. 79, 181–211 (2011).
Davis, A. J., Chen, B. P. C. & Chen, D. J. DNA-PK: A dynamic enzyme in a versatile DSB repair pathway. DNA Repair (Amst). 17, 21–29 (2014).
Simsek, D. & Jasin, M. Alternative end-joining is suppressed by the canonical NHEJ component Xrcc4-ligase IV during chromosomal translocation formation. Nat. Struct. Mol. Biol. 17, 410–416 (2010).
Kent, T., Chandramouly, G., Mcdevitt, S. M., Ozdemir, A. Y. & Pomerantz, R. T. Mechanism of microhomology-mediated end-joining promoted by human DNA polymerase θ. Nat. Struct. Mol. Biol. 22, 230–237 (2015).
Schimmel, J., van Schendel, R., den Dunnen, J. T. & Tijsterman, M. Templated insertions: A smoking gun for polymerase theta-mediated end joining. Trends Genet. 35, 632–644 (2019).
Suzuki, K. et al. In vivo genome editing via CRISPR/Cas9 mediated homology-independent targeted integration. Nature 540, 144–149 (2016).
Nakade, S. et al. Microhomology-mediated end-joining-dependent integration of donor DNA in cells and animals using TALENs and CRISPR/Cas9. Nat. Commun. 5, 5560 (2014).
Iiizumi, S. et al. Impact of non-homologous end-joining deficiency on random and targeted DNA integration: Implications for gene targeting. Nucleic Acids Res. 36, 6333–6342 (2008).
Saito, S., Maeda, R. & Adachi, N. Dual loss of human POLQ and LIG4 abolishes random integration. Nat. Commun. 8, 16112 (2017).
Zelensky, A. N., Schimmel, J., Kool, H., Kanaar, R. & Tijsterman, M. Inactivation of Pol θ and C-NHEJ eliminates off-target integration of exogenous DNA. Nat. Commun. 8, 66 (2017).
Kim, S., Kim, D., Cho, S. W., Kim, J. & Kim, J. S. Highly efficient RNA-guided genome editing in human cells via delivery of purified Cas9 ribonucleoproteins. Genome Res. 24, 1012–1019 (2014).
Yang, H. et al. One-step generation of mice carrying reporter and conditional alleles by CRISPR/Cas-mediated genome engineering. Cell 154, 1370-1379 (2013).
Miyaoka, Y. et al. Systematic quantification of HDR and NHEJ reveals effects of locus, nuclease, and cell type on genome-editing. Sci. Rep. 6, 23549 (2016).
Supharattanasitthi, W., Carlsson, E., Sharif, U. & Paraoan, L. CRISPR/Cas9-mediated one step bi-allelic change of genomic DNA in iPSCs and human RPE cells in vitro with dual antibiotic selection. Sci. Rep. 9, 174 (2019).
Jarazo, J., Qing, X. & Schwamborn, J. C. Guidelines for fluorescent guided biallelic HDR targeting selection with PiggyBac system removal for gene editing. Front. Genet. 10, 190 (2019).
Yeh, C. D., Richardson, C. D. & Corn, J. E. Advances in genome editing through control of DNA repair pathways. Nat. Cell Biol. 21, 1468–1478 (2019).
Liu, M. et al. Methodologies for improving HDR efficiency. Front. Genet. 10, 691 (2019).
Bischoff, N., Wimberger, S., Maresca, M. & Brakebusch, C. Improving precise CRISPR genome editing by small molecules: Is there a magic potion? Cells 9, 1318 (2020).
Chu, V. T. et al. Increasing the efficiency of homology-directed repair for CRISPR-Cas9-induced precise gene editing in mammalian cells. Nat. Biotechnol. 33, 543–548 (2015).
Harnor, S. J., Brennan, A. & Cano, C. Targeting DNA-dependent protein kinase for cancer therapy. ChemMedChem 12, 895–900 (2017).
Riesenberg, S. et al. Simultaneous precise editing of multiple genes in human cells. Nucleic Acids Res. 47, e116 (2019).
Fu, Y.-W. et al. Dynamics and competition of CRISPR–Cas9 ribonucleoproteins and AAV donor-mediated NHEJ, MMEJ and HDR editing. Nucleic Acids Res. 49, 969–985 (2021).
Abadi, S., Yan, W. X., Amar, D. & Mayrose, I. A machine learning approach for predicting CRISPR-Cas9 cleavage efficiencies and patterns underlying its mechanism of action. PLoS Comput. Biol. 13, e1005807 (2017).
Li, J. et al. A dominant-negative form of mouse SOX2 induces trophectoderm differentiation and progressive polyploidy in mouse embryonic stem cells. J. Biol. Chem. 282, 19481–19492 (2007).
Zhou, J. et al. A first-in-class polymerase theta inhibitor selectively targets homologous-recombination-deficient tumors. Nat. Cancer 2, 598–610 (2021).
Zhang, J. P. et al. Efficient precise knockin with a double cut HDR donor after CRISPR/Cas9-mediated double-stranded DNA cleavage. Genome Biol. 18, 35 (2017).
Yao, X. et al. Homology-mediated end joining-based targeted integration using CRISPR/Cas9. Cell Res. 27, 801–814 (2017).
Wierson, W. A. et al. Efficient targeted integration directed by short homology in zebrafish and mammalian cells. Elife 9, e53968 (2020).
Wang, H. & Xu, X. Microhomology-mediated end joining: New players join the team. Cell Biosci. 7, 6 (2017).
Aida, T. et al. Gene cassette knock-in in mammalian cells and zygotes by enhanced MMEJ. BMC Genomics 17, 979 (2016).
Zhou, Y., Caron, P., Legube, G. & Paull, T. T. Quantitation of DNA double-strand break resection intermediates in human cells. Nucleic Acids Res. 42, e19 (2014).
Owens, D. D. G. et al. Microhomologies are prevalent at Cas9-induced larger deletions. Nucleic Acids Res. 47, 7402–7417 (2019).
Hsieh, T. & Brutlag, D. ATP-dependent DNA topoisomerase from D. melanogaster reversibly catenates duplex DNA rings. Cell 21, 115–125 (1980).
Marcu, M. G., Schulte, T. W. & Neckers, L. Novobiocin and related coumarins and depletion of heat shock protein 90-dependent signaling proteins. J. Natl. Cancer Inst. 92, 242–248 (2000).
Schrempf, A., Slyskova, J. & Loizou, J. I. Targeting the DNA repair enzyme polymerase θ in cancer therapy. Trends Cancer 7, 98–111 (2021).
Bressan, R. B. et al. Efficient CRISPR/Cas9-assisted gene targeting enables rapid and precise genetic manipulation of mammalian neural stem cells. Development 144, 635–648 (2017).
Yesbolatova, A., Natsume, T., Hayashi, K. & Kanemaki, M. T. Generation of conditional auxin-inducible degron (AID) cells and tight control of degron-fused proteins using the degradation inhibitor auxinole. Methods 164–165, 73–80 (2019).
Arai, D. et al. An epigenetic regulatory element of the Nodal gene in the mouse and human genomes. Mech. Dev. 136, 143–154 (2015).
Tanaka, T. S., Davey, R. E., Lan, Q., Zandstra, P. W. & Stanford, W. L. Development of a gene-trap vector with a highly sensitive fluorescent protein reporter system for expression profiling. Genesis 46, 347–356 (2008).
Tamm, C., Kadekar, S., Pijuan-Galitó, S. & Annerén, C. Fast and efficient transfection of mouse embryonic stem cells using non-viral reagents. Stem Cell Rev. Rep. 12, 584–591 (2016).
Clement, K. et al. CRISPResso2 provides accurate and rapid genome editing sequence analysis. Nat. Biotechnol. 37, 224–226 (2019).
We thank Dr. Jun Ohgane for providing the shRNA expression vector, Dr. Tetsuya S. Tanaka for providing the IRES-Venus containing vector, Drs. Makoto Miyagishi and Hideo Akashi for providing the pENTR vector, Dr. Feng Zhang for providing the pX330 vector, Dr. Frank Costantini for providing the pROSA26-PA vector, Dr. Phil Sharp for providing pCAGGS-mCherry, and Dr. Masato Kanemaki for providing the pMK391 vector. We thank Jeremy Allen, PhD, from Edanz (https://jp.edanz.com/ac) for editing a draft of this manuscript. This work was supported by JSPS Grants-in-Aid for Scientific Research, Grant Numbers 20K06449, 18H03993, 18H02100, 26221204, and a Waseda University Grant for Special Research Projects (2020C-289).
The authors declare no competing interests.
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Arai, D., Nakao, Y. Efficient biallelic knock-in in mouse embryonic stem cells by in vivo-linearization of donor and transient inhibition of DNA polymerase θ/DNA-PK. Sci Rep 11, 18132 (2021). https://doi.org/10.1038/s41598-021-97579-8
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