Abstract
Gene conversion is a specific form of homologous recombination (HR), involving the unidirectional transfer of genetic information from one genomic locus to another. CRISPR-Cas9-directed double strand breaks (DSBs) induce both interallelic and interlocus gene conversion in early human embryos and somatic cells, suggesting its potential for correcting pathogenic mutations. However, the key features in mitotic gene conversion, including its efficiency, the length of conversion track, and its dependency on specific recombination proteins, remain largely undefined. Here, we show that allele-specific CRISPR-Cas9-induced DSBs, without exogenous donor templates, can efficiently correct a heterozygous pathogenic variant (c.1582C>T; p.Arg528Trp) in the ATAD3A gene of patient-derived induced pluripotent stem cells (iPSCs). Amplicon-based next-generation sequencing (NGS) revealed that approximately 38%~53% of edited iPSCs carried two wild-type ATAD3A alleles. Notably, over 99% of the corrected alleles derived from the homologous chromosome, indicating that the repair occurred mainly via interallelic gene conversion. Long-range amplicon nanopore sequencing coupled with haplotype analysis showed that the majority of gene conversion tracts was less than 2 kilobases in length. Whole-genome sequencing of three corrected iPSC clones showed the absence of large deletions or structural rearrangements at the ATAD3A target site. However, one clone carried a heterozygous deletion in ATAD3B locus, suggesting that CRISPR-Cas9 can introduce off-target genomic alterations. Knockdown of key HR proteins, including RAD51, CtIP, and BRCA1/2, significantly reduced the correction efficiency, indicating that the gene conversion relies on a RAD51-dependent HR pathway. Together, our findings provide compelling evidence that template-free CRISPR-Cas9-mediated interallelic gene conversion can be harnessed to correct disease causing variants in human iPSCs.