<?xml version="1.0" encoding="utf-8"?>
    <rss version="2.0">
      <channel xmlns:content="http://purl.org/rss/1.0/modules/content/">
        <title>Frontiers in Genome Editing | New and Recent Articles</title>
        <link>https://www.frontiersin.org/journals/genome-editing</link>
        <description>RSS Feed for Frontiers in Genome Editing | New and Recent Articles</description>
        <language>en-us</language>
        <generator>Frontiers Feed Generator,version:1</generator>
        <pubDate>2026-05-03T15:22:05.371+00:00</pubDate>
        <ttl>60</ttl>
        <item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2026.1762449</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2026.1762449</link>
        <title><![CDATA[Reconstructing the complex architecture of the genome with molecular scissors: applying genome editing technology in precision medicine]]></title>
        <pubdate>2026-04-30T00:00:00Z</pubdate>
        <category>Review</category>
        <author>Md Nur Amin Khan</author><author>Rohit Das</author><author>Pooja Barik</author><author>Somasundaram Arumugam</author><author>Shiladitya Chattopadhyay</author>
        <description><![CDATA[Our past, present, and future are governed by the grand design of the genetic blueprint, which was mapped more than two decades back. While the eloquent design of our genome results from millions of years of evolution and has reached a near-perfect stage, unwanted flaws and mistakes in individual genomes can make their life miserable and worth intervention. The advent of technologies to manipulate the grand design and make it congenial for the individual has given new hope. Here, we discuss how gene editing technologies have progressed and how some of the technologies have become indispensable gears in precision medicine.]]></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2026.1803282</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2026.1803282</link>
        <title><![CDATA[Commentary: CRISPR-Cas9 mediated editing of starch branching enzyme, SBE2 gene in potato for enhanced resistant starch for health benefits]]></title>
        <pubdate>2026-04-22T00:00:00Z</pubdate>
        <category>General Commentary</category>
        <author>Ling Yin</author>
        <description></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2026.1789952</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2026.1789952</link>
        <title><![CDATA[Advances in gene editing for legume improvement: technologies, progress, and prospects]]></title>
        <pubdate>2026-04-15T00:00:00Z</pubdate>
        <category>Review</category>
        <author>Shallu Thakur</author><author>Shalini Pareek</author><author>G. P. Dixit</author><author>Geoffrey Meru</author><author>Alok Das</author>
        <description><![CDATA[Legumes are among the most important protein-rich crops in global agri-food systems. To meet the rising protein demand of a growing population, significant efforts are underway to enhance legume yield, nutritional quality, and resilience to environmental stresses through the manipulation of key genetic traits. Advanced technologies-including genetic engineering, gene editing, genomic selection, next-generation sequencing, single-cell genomics, and multi-omics-are accelerating legume improvement due to their high precision and efficiency. This review focuses on major gene-editing technologies, namely, CRISPR/Cas9 (Clustered Regularly Interspaced Short Palindromic Repeats/CRISPR-associated protein 9), TALENs (Transcription Activator-Like Effector Nucleases), ZFNs (Zinc Finger Nucleases), base editing (BE), and prime editing (PE), and their applications in key legume crops such as soybean (Glycine max), cowpea (Vigna unguiculata), chickpea (Cicer arietinum), groundnut (Arachis hypogaea), pea (Pisum sativum), barrel clover (Medicago truncatula), alfalfa (Medicago sativa), and Lotus japonicus. Among these platforms, CRISPR/Cas9 is the most widely adopted in legumes, largely due to its simplicity, versatility, and dependence on accurate genome sequence information and guide RNA (gRNA) design. Advances in next-generation sequencing and the growing availability of intuitive online gRNA design tools have streamlined CRISPR workflows, improving accessibility and precision. The present review indicates that CRISPR-P is the most used gRNA design tool in legume research, likely due to its early development for plant systems and integrated off-target prediction features. Therefore, alongside reviewing gene-editing applications, we emphasized the critical role of robust gRNA design tools as a foundation for successful genome editing. Future integration of artificial intelligence and large language models is expected to further enhance target prediction accuracy, minimize off-target effects, and enable more precise genome-editing strategies in legumes.]]></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2026.1777148</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2026.1777148</link>
        <title><![CDATA[Development of in planta genome editing by transient expression of genome-editing tools in tomato]]></title>
        <pubdate>2026-04-09T00:00:00Z</pubdate>
        <category>Original Research</category>
        <author>Misaki Kobayashi</author><author>Na Renhu</author><author>Shu Takahashi</author><author>Seungje Choi</author><author>Haruto Watanabe</author><author>Martina Bianca Fuhrmann-Aoyagi</author><author>Hiroshi Ezura</author><author>Kenji Miura</author>
        <description><![CDATA[Two major processes are important for genome editing in plants: transformation by stable transfection, in which nucleic acids encoding genome-editing enzymes are introduced into plant cells and the regeneration of plant individuals from cells harboring mutations by genome-editing enzymes. The efficiency of transformation and regeneration by tissue culture varies across plant species, and is low in some practical crop species. In planta methods have been developed to exclude the need for tissue culture. However, few reports are available on methods that do not require stable transfection. Therefore, this study aimed to develop a new protocol for delivery genome editing tools that does not require transformation or tissue culture, by combining the in planta method with transient genome editing tools instead of stable transfection. Cas9, guide RNAs, and developmental regulators, which are factors involved in mitotic tissue induction, were transiently expressed by agroinfiltration of the stem tissue cut surfaces of tomatoes. New chimeric mutants, containing a mixture of cells with mutations introduced at or near the target sequence, were obtained. After examining conditions such as the concentration of Agrobacterium used for infection and post-infection treatment, we succeeded in obtaining chimeric mutants with an efficiency of 11.7%. In addition, most of the observed mutations were single base substitutions. These results indicate that the in planta method with transient expression of genome editing tools and induction of meristematic tissue can be used to introduce genome-edited mutations in tomatoes.]]></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2026.1813338</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2026.1813338</link>
        <title><![CDATA[Editorial: Genome editing strategies for augmenting crop resilience against climate change]]></title>
        <pubdate>2026-03-13T00:00:00Z</pubdate>
        <category>Editorial</category>
        <author>Wadzani Palnam Dauda</author><author>Amolkumar U. Solanke</author><author>Ramesh Namdeo Pudake</author>
        <description></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2026.1749445</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2026.1749445</link>
        <title><![CDATA[Harnessing myostatin pleiotropy for multitrait improvement via precision gene editing]]></title>
        <pubdate>2026-03-12T00:00:00Z</pubdate>
        <category>Review</category>
        <author>Yajun Chen</author><author>Ruiyao Yang</author><author>Yucai Yang</author><author>Qianguang Wang</author><author>Kai Yang</author><author>Man Xu</author>
        <description><![CDATA[The pursuit of sustainable livestock farming to meet the rising global protein demand has positioned myostatin (MSTN) gene editing as a key technology. However, the field’s focus on the remarkable double-muscle phenotype has often overshadowed a systematic examination of its concomitant effects. The present review aims to bridge this gap by moving beyond a singular focus on productivity. First, the pleiotropic effects of MSTN gene editing on growth performance, carcass quality, and meat quality in cattle, swine, sheep, poultry, and aquatic species were comprehensively evaluated. Next, the cascading biological effects of MSTN editing on metabolic homeostasis, reproductive performance, and animal health and welfare werAAe analyzed in depth. Finally, the inherent limitations and ethical issues of current editing techniques were critically discussed, and future sustainable breeding programs aimed at balanced multitrait regulation were prospectively proposed. Ultimately, this review affirms that MSTN editing has a multiplicative effect on trait alterations; however, there is also a series of associated health challenges, which demonstrates that the technology’s impact is systemic, generating a spectrum of trade-offs that are often species specific. Its responsible application therefore hinges on multitrait balancing strategies to simultaneously secure productivity and sustainability in animal agriculture.]]></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2026.1718252</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2026.1718252</link>
        <title><![CDATA[The precision strategy of human genome correction via a set of circular donor DNA and its cleaver]]></title>
        <pubdate>2026-03-11T00:00:00Z</pubdate>
        <category>Original Research</category>
        <author>Kohji Kusano</author><author>Kaoru Takizawa</author><author>Jitsutaro Kawaguchi</author><author>Isamu Hara</author><author>Toyotaka Mori</author>
        <description><![CDATA[Homologous recombination (HR) corrects a mutational sequence causing a genetic disease by replacing it with the normal sequence to restore a healthy state in humans. A targeted genomic breakage, such as that induced by CRISPR–Cas9, can trigger a copy-paste-type HR event; however, CRISPR–Cas9 more frequently induces imprecise non-homologous end-joining events, leading to one-step multiple knockout products for paralogous genes or homologous alleles, which can be considered a unique advantage. We have established a precision strategy for crossover-type HR-based gene editing, primed by intra-cellular circular donor cleavage (InCDC). The InCDC technique generates targeted duplication of the circular donor plasmid at the target locus in human cells, forming a doublet configuration comprising the donor DNA with the designed sequence and the target DNA with the original sequence, with much higher efficiency than conventional donor linearization techniques. This doublet form leads to the singlet form, resulting in retention of the designed allele. We found that the safety distance within the designed circular donor plasmid and its intra-cellular cleavage was particularly critical to protect a designed sequence from enzymatic exclusion, and we propose that InCDC technology enables precision genome editing, such as the replacement of a genetic disease-causing allele with the correctly designed allele.]]></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2026.1755922</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2026.1755922</link>
        <title><![CDATA[CRISPR/Cas9-mediated knockout of DFR alters pigmentation and shifts flavonoid accumulation in red leaf lettuce without detectable growth penalties]]></title>
        <pubdate>2026-03-04T00:00:00Z</pubdate>
        <category>Original Research</category>
        <author>Ai Nagamine</author><author>Masaki Ono</author><author>Osuke Sato</author><author>Eiji Goto</author><author>Hiroshi Ezura</author>
        <description><![CDATA[Red leaf lettuce (Lactuca sativa L. cv. ‘Red Fire’) is a preferred crop in plant factories with artificial light (PFALs) due to its short cultivation cycle and high anthocyanin content, which increases both its nutritional value and visual appeal. However, anthocyanins strongly influence leaf coloration and antioxidant profiles, and their levels are highly responsive to the light environment. Therefore, targeted editing of flavonoid biosynthesis may provide a breeding strategy to diversify pigment composition and associated functional traits under PFAL conditions. In this study, we used CRISPR/Cas9 to knock out DFR (dihydroflavonol 4-reductase), a key enzyme in the anthocyanin pathway. Genome-edited lines were generated via a dual-guide RNA system, resulting in a successfully edited red leaf genotype. The DFR-knockout lines displayed a complete loss of red pigmentation and a visibly distinct green phenotype. Metabolite profiling revealed a significant decrease in anthocyanin levels, accompanied by an increase in total flavonoid levels in some lines. Growth traits, including shoot dry weight and leaf number, were not significantly affected, suggesting that DFR knockout does not compromise growth under PFAL conditions. These findings highlight DFR as a promising target for creating pigment-altered lettuce lines for controlled-environment cultivation, including PFAL systems.]]></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2026.1705463</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2026.1705463</link>
        <title><![CDATA[Evaluation of genetic variation in tumor suppressor miRNA encoding and their target genes in breast cancer; focus on miRNA interaction and expression analysis]]></title>
        <pubdate>2026-02-27T00:00:00Z</pubdate>
        <category>Original Research</category>
        <author>Yogita Chhichholiya</author><author>Sandeep Singh</author><author>Rajesh Vashistha</author><author>Manjit Kaur Rana</author><author>Anjana Munshi</author>
        <description><![CDATA[BackgroundGenetic variations in tumor suppressor miRNAs and the 3′UTR of their target genes influence tumor biology and breast cancer (BC) risk.ObjectiveThis study investigated genetic variations in tumor suppressor miRNAs (hsa-let-7c, hsa-miR-34a, hsa-miR-145a) and their target genes (KRAS, IGFBP6, IGF1R), and their functional significance in BC patients.MethodsThe miRNA encoding regions and 3′UTRs of the selected target genes were sequenced in 208 BC patients. Functional analyses were performed using luciferase assay, RT-PCR, IHC, and Western blotting. RNAfold, TNM plot, Kaplan-Meier Plotter, and ROC Plotter were used for structural predictions, survival, and therapy response analysis.ResultsTwo variants, rs712 and rs9266, were found in the 3′UTR of KRAS. Luciferase assay confirmed that rs9266 disrupts the binding of hsa-let-7c and hsa-miR-181c, leading to increased KRAS expression. KRAS expression was highest in heterozygous, followed by homozygous mutant, and lowest in wild-type genotypes. Higher hsa-let-7c and hsa-miR-181c expression correlated with better survival. ROC analysis identified KRAS as a potential predictive biomarker for chemotherapy response.ConclusionVariants rs712 and rs9266 in the KRAS 3′UTR impair miRNA binding, enhancing KRAS expression and tumorigenesis, while elevated hsa-let-7c and hsa-miR-181c levels predict favourable survival outcomes in BC patients.]]></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2026.1787940</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2026.1787940</link>
        <title><![CDATA[Correction: Diversity of transgene integration and gene-editing events in wheat (Triticum aestivum L.) transgenic plants generated using Agrobacterium-mediated transformation]]></title>
        <pubdate>2026-02-19T00:00:00Z</pubdate>
        <category>Correction</category>
        <author>Louie Cris Lopos</author><author>Natalia V. Bykova</author><author>Janeen Robinson</author><author>Susan Brown</author><author>Kerry Ward</author><author>Andriy Bilichak</author>
        <description></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2025.1729535</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2025.1729535</link>
        <title><![CDATA[CRISPR/Cas9-based programmable genome editing in chickens: concepts, applications and regulatory issues]]></title>
        <pubdate>2026-01-09T00:00:00Z</pubdate>
        <category>Review</category>
        <author>Gautham Kolluri</author><author>Adnan Naim</author><author>Shiva Kumar Kurva</author><author>Jagbir Singh Tyagi</author><author>Mohd. Matin Ansari</author><author>Simmi Tomar</author><author>Ashok Kumar Tiwari</author><author>Laxmi Chouhan</author>
        <description><![CDATA[The advent of genetics, molecular biology, and genome sequencing has rapidly accelerated the development of elite genetic lines across various species, including poultry. It is now possible to introduce intra- or inter-species single nucleotide polymorphisms into chicken lines to enhance productivity. This advancement may mark the beginning of a new agricultural revolution, dramatically reducing the time required to improve poultry lines for commercial production environments. Transgenic technologies, including lentiviral vectors and piggyBac transposition, have enabled the generation of animals expressing exogenous genes. The emergence of new genome-editing tools is transforming avian biotechnology, allowing the creation of customized organisms for specific traits. Genome editing has become the most efficient method for studying gene function. First and second generation tools, such as zinc finger nucleases and transcription activator-like effector nucleases (TALENs), are limited by complex design and off-target effects. In contrast, the third generation Clustered Regularly Interspaced Short Palindromic Repeats/CRISPR-associated protein 9 (CRISPR/Cas9), represents a significant breakthrough. It encompasses guided RNA (gRNA) and the Cas9 endonuclease which together target specific DNA sequences and induces double-strand breaks that are repaired via error-prone non-homologous end joining, frequently causing insertions or deletions that disrupt gene function. Targeting specificity is achieved through gRNA-DNA base pairing and recognition of a protospacer adjacent motif by Cas9. Beyond gene knockout, CRISPR/Cas9 enables functional analysis of non-coding elements such as enhancers and insulators. Delivered via plasmid systems, Cas9 and gRNA are transiently expressed and degrade within 48–72 h, leaving no permanent genetic footprint. Since no exogenous DNA is integrated, this approach is generally considered less contentious than traditional transgenic methods in the context of genetically modified organism regulation. CRISPR/Cas9 has diverse applications in poultry, including enhancing disease resistance to avian influenza and Marek’s disease, improving productivity traits such as growth, feed efficiency, and egg-laying, and enabling early in-ovo sexing to address ethical concerns around male chick culling. It also allows control of reproductive traits for breeding management, supports bio-pharming by producing therapeutic proteins or vaccines in eggs, and facilitates functional genomics through precise gene knockouts to study development, immunity, and metabolism.]]></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2025.1724291</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2025.1724291</link>
        <title><![CDATA[Therapeutic applications of CRISPR-Cas9 gene editing]]></title>
        <pubdate>2025-12-16T00:00:00Z</pubdate>
        <category>Mini Review</category>
        <author>Aditya Bharti</author><author>Joann Mudge</author>
        <description><![CDATA[CRISPR-Cas9 is a gene editing tool used extensively in biological research that is now making its way into clinical therapies. With the first CRISPR therapy obtaining approval by the United States’ Food and Drug Administration (FDA) in late 2023, we look at clinical trials of emerging therapies involving CRISPR-Cas9, currently the most prevalent CRISPR-based tool in these trials. A CRISPR-based therapy is currently approved for treatment of both sickle-cell anemia and transfusion-dependent β-thalassemia but clinical trials for CRISPR-based therapeutics include a much broader range of targets. CRISPR-Cas9 is being explored to treat cancer, infectious disease, and more. This review highlights CRISPR-Cas9 clinical trials registered at clinicaltrials.gov as of 12/31/2024.]]></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2025.1588089</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2025.1588089</link>
        <title><![CDATA[Emerging tools in plant genome editing]]></title>
        <pubdate>2025-12-04T00:00:00Z</pubdate>
        <category>Review</category>
        <author>Shilpi Sharma</author><author>Naveen Kumar Saroha</author><author>Abhilasha Sehrawat</author><author>Guiliang Tang</author><author>Deepali Singh</author><author>Sachin Teotia</author>
        <description><![CDATA[Plant genome editing has undergone a transformative shift with the advent of advanced molecular tools, offering unprecedented levels of precision, flexibility and efficiency in modifying genetic material. While classical site-directed nucleases such as ZFNs, TALENs and CRISPR-Cas9 have revolutionized genome engineering by enabling targeted mutagenesis and gene knockouts, the landscape is now rapidly evolving with the emergence of novel systems that go beyond the conventional double strand break (DSB)-mediated approaches. Advanced and recent tools include LEAPER, SATI, RESTORE, RESCUE, ARCUT, SPARDA, helicase-based approaches like HACE and Type IV-A CRISPR system, and transposon-based techniques like TATSI and piggyBac. These tools unlock previously inaccessible avenues of genome and transcriptome modulation. Some of these technologies allow DSB-free editing of DNA, precise base substitutions and RNA editing without altering the genomic DNA, a significant advancement for regulatory approval and for species with complex genomes or limited regeneration capacity. While LEAPER, RESCUE and RESTORE are the new advents in the RNA editing tool, SATI allows DSB-free approach for DNA editing, ARCUT offers less off-target and cleaner DNA repairs and Type IV-A CRISPR system induces gene silencing rather than editing. The transposon-based approaches include TATSI, piggyBac and TnpB, and helicases are used in HACE and Type IV-A CRISPR system. The prokaryotic Argonaute protein is used in SPARDA tool as an endonuclease to edit DNA. The transient and reversible nature of RNA editing tools such as RESTORE and LEAPER introduces a new layer of epigenetics-like control in plant systems, which could be harnessed for tissue-specific and environmentally-responsive trait expression. Simultaneously, innovations like ARCUT and SPARDA utilize chemically-guided editing, minimizing reliance on biological nucleases and reducing off-target risks. Their modularity and programmability are enabling gene function studies, synthetic pathway designs and targeted trait stacking. These advances represent a novel synthesis of genome engineering and systems biology, positioning plant genome editing not just as a tool of modification but as a platform for designing adaptive and intelligent crops, tailored to future environmental and nutritional challenges. Although, many of these recent tools remain to be applied on plant systems, they are proven to be effective elsewhere and hold a great potential to be effective in creating climate-resilient crops.]]></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2025.1713347</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2025.1713347</link>
        <title><![CDATA[Development of efficient targeted insertion mediated by CRISPR-Cas12a and homology-directed repair in maize]]></title>
        <pubdate>2025-12-04T00:00:00Z</pubdate>
        <category>Original Research</category>
        <author>Brenden Barco</author><author>Shujie Dong</author><author>Yuki Matsuba</author><author>Ashley Crook</author><author>Ruiji Xu</author><author>Yingxiao Zhang</author><author>Chengjin Zhang</author><author>Ryan Carlin</author><author>Kevin Potter</author><author>Stephen B. Rigoulot</author><author>Jeongmoo Park</author><author>Erin M. Seaberry</author><author>Allison Parrish</author><author>Sivamani Elumalai</author><author>Sam Nalapalli</author><author>Craig Schuller</author><author>Anna Prairie</author><author>Anna Mangum</author><author>Kangfeng Mei</author><author>Hao Wu</author><author>Melissa Murray</author><author>Kristin Setliff</author><author>Francine Johnson</author><author>Dawn McNamara</author><author>Ling Zhu</author><author>Mark Rose</author><author>Weining Gu</author><author>Hao Hu</author><author>Yuanji Zhang</author><author>Yaping Jiang</author><author>Wenling Wang</author><author>Guozhu Tang</author><author>Lizhao Geng</author><author>Jianping Xu</author><author>Wan Shi</author><author>Jason Nichols</author><author>Tim Kelliher</author><author>Liang Shi</author><author>Ian Jepson</author><author>Qiudeng Que</author>
        <description><![CDATA[Targeted insertion (TIN) of transgenic trait cassettes has the potential to reduce timeline and cost for GM product development and commercialization. Precise genome engineering has made remarkable progress over the last several decades, particularly with the use of site-directed nucleases as core editing machinery. However, there are still many critical factors that can impact TIN efficiency including insertion site selection, nuclease optimization and expression, donor vector design, gene delivery, and stable event regeneration. Here, we develop workflows for target site sequence identification and gRNA screening for CRISPR-Cas12a system and demonstrate its successful application for TIN in maize with donor sequences up to 10 kilobase pairs (kb) in size. We first prioritize genomic regions for inserting transgenes in silico using bioinformatics tools and then test gRNA performance using a leaf protoplast transient assay. Despite its known low efficiency, we identify homology-directed repair (HDR) as the preferential pathway for directing targeted insertions of large sequences in immature embryos and demonstrate double-junction integrations at a rate of up to 4%. We further apply a molecular analysis workflow using large amplicon TaqMan assays and nanopore sequencing for streamlined identification and characterization of high-quality insertion events with intact large inserts. Analysis of TIN events across generations suggests that efficiency bottlenecks are not limited to donor targeted integration; attrition in efficiency also results from partial or additional donor insertion, chimerism, and close linkage with undesired sequence insertions such as those encoding the editing machinery. This work represents a major step forward in realizing the potential of precise genome engineering in maize for basic research and biotech trait development applications.]]></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2025.1686412</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2025.1686412</link>
        <title><![CDATA[CRISPR-Cas9 mediated editing of starch branching enzyme, SBE2 gene in potato for enhanced resistant starch for health benefits]]></title>
        <pubdate>2025-11-26T00:00:00Z</pubdate>
        <category>Original Research</category>
        <author>Sudha Batta</author><author>Sundaresha Siddappa</author><author>Neha Sharma</author><author>Rajender Singh</author><author>Reena Gupta</author><author>Dinesh Kumar</author><author>Brajesh Singh</author><author>Ajay Kumar Thakur</author>
        <description><![CDATA[Potato is an important vegetatively propagated, starch-rich tuber crop. High amylose potatoes containing more resistant starch offer healthier food alternatives. However, the resistant starch content is low in most cultivated potato varieties. In this study, targeted mutation of the starch branching enzyme2 (SBE2.1 & SBE2.2 isoforms) had been done in the commercially significant potato cultivar, Kufri Chipsona-I using Clustered regularly interspaced short palindromic repeats-CRISPR-associated protein 9 (CRISPR-Cas9 system) to develop high-amylose potato lines. SBE2 is one of the key enzymes involved in amylopectin biosynthesis, a starch component. Two isoforms, SBE2.1 & SBE2.2, were mutated using CRISPR-Cas9-mediated genome editing. After Agrobacterium-mediated genetic transformation, fifty transformed lines were generated on herbicide Basta selection medium, out of which 70% were found positive for bar and Cas9 genes. Overall, six mutant lines, viz. K301, K302, K303, K304, K305, K306, derived from distinct events, exhibited deletions and substitutions in the target exons. The CRISPR-Cas9 edited K304 potato line exhibited both insertion–deletion (indel) and substitution mutations in three out of the four selected targets across both genes, and was therefore identified as the most efficiently edited line. The harvested tubers from SBE2.1 & SBE2.2 mutant K304 line showed the highest amylose (95.91%) and resistant starch content (8.69 g/100 g). Evaluation of starch using X-ray crystallography (XRD) illustrated an altered crystallinity index (CI%) in all six mutant events in comparison to the wild study. Furthermore, 1H-NMR study demonstrated a substantial decline in branch chain elongation in amylopectin, and thus a low degree of branching in a range of 1.15%–3.66% was reported in mutant lines, relative to the wild type (5.46%). The present study demonstrated the efficacy of CRISPR-Cas9-mediated mutagenesis of starch biosynthetic genes to develop high-amylose potato lines with elevated resistant starch content for improved health benefits.]]></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2025.1740380</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2025.1740380</link>
        <title><![CDATA[Editorial: Social aspects of crop genome editing]]></title>
        <pubdate>2025-11-25T00:00:00Z</pubdate>
        <category>Editorial</category>
        <author>Srividhya Venkataraman</author><author>Kathleen Hefferon</author>
        <description></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2025.1679698</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2025.1679698</link>
        <title><![CDATA[Construction of EpCAM overexpression and knockdown vectors and their implications in colorectal cancer research]]></title>
        <pubdate>2025-11-20T00:00:00Z</pubdate>
        <category>Original Research</category>
        <author>Bingping Wang</author><author>Jinkai Duan</author><author>Jie Zhou</author><author>Hulin Ma</author><author>Meng Ren</author><author>Liangquan Chen</author><author>Rina Su</author><author>Hao Zhang</author><author>Shuang Zhang</author><author>Yanwei Gao</author>
        <description><![CDATA[BackgroundThe functional characterization of Epithelial Cell Adhesion Molecule (EpCAM) in colorectal cancer (CRC) progression has been constrained by methodological limitations, particularly the potential for truncated protein isoforms to confound traditional genetic knockout approaches. This study aimed to develop a novel CRISPR/Cas9 strategy to overcome this challenge and systematically elucidate the context-dependent oncogenic roles of EpCAM across diverse CRC models.MethodsWe engineered EpCAM overexpression (pCDH-EpCAM) and CRISPR/Cas9 knockdown (pGMC-KO-EpCAM) vectors using restriction digestion and T4 DNA ligation. A strategic dual-exon targeting approach (exons 1 and 3) was employed to minimize the risk of functional escape variants. Selected CRC cell lines (HT-29, HT-115, HRT-18) were genetically modified using optimized Lipofectamine 2000 transfection. Functional impacts were quantitatively assessed through: (i) flow cytometry for EpCAM surface expression (CD326-PE); (ii) daily cell counting over 8 days for proliferation kinetics; and (iii) scratch wound healing (0/24/48 h) and Transwell migration assays (8-μm pores, 18 h) to evaluate metastatic potential.ResultsSuccessful genetic modulation was achieved and validated: HT-29-OE-EpCAM-2 exhibited an 89% EpCAM-positive rate versus 12% in wild-type (WT) (*p*<0.001), while HRT-18-KD-EpCAM-3 showed a significant reduction to 4% EpCAM-positive cells (vs. 15% in WT, *p*<0.001). EpCAM overexpression accelerated proliferation, with HT-29-OE cells showing a 20.1% increase in peak density on day 5 (30.76 ± 0.15 × 104 vs. WT 25.62 ± 0.25 × 104; *p*<0.001). Conversely, EpCAM knockdown in HRT-18 cells prolonged the doubling time by 8.8% (30.8 h vs. WT 28.3 h; *p*<0.05). Migration capacity was profoundly altered: HT-115-OE cells achieved complete scratch closure (100% vs. 74.05% in WT, *p*<0.001), whereas HRT-18-KD cells showed an 80.5% reduction (*p*<0.001). Transwell migration hierarchy confirmed the pro-metastatic role of EpCAM (HT-29-OE > HT-115-OE > HRT-18-KD; ANOVA *p* = 0.0024).ConclusionThis study establishes a robust dual-vector toolkit for reliable EpCAM manipulation, highlighting a novel exon-targeting strategy that mitigates the limitations of previous approaches. Our findings demonstrate that EpCAM is a master regulator of CRC aggressiveness, dictating proliferative and metastatic phenotypes in a cell context-dependent manner. The genetically defined models provide a validated platform for therapeutic screening and safety assessment, forming a foundational resource for advancing EpCAM-targeted therapies and diagnostic applications.]]></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2025.1663352</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2025.1663352</link>
        <title><![CDATA[A long journey towards genome editing technologies in plants: a technical and critical review of genome editing technologies]]></title>
        <pubdate>2025-11-11T00:00:00Z</pubdate>
        <category>Review</category>
        <author>Dylan Gallo</author><author>Anne-Cécile Meunier</author><author>Christophe Périn</author>
        <description><![CDATA[Advancements in genome editing technologies, notably CRISPR/Cas9, base editing (BE), and prime editing (PE), have revolutionized plant biotechnology, offering unprecedented precision in crop improvement to address the ongoing global warming challenge. This review provides a critical analysis of recent developments in SpCas9-based editing tools, emphasizing enhancements in editing efficiency and specificity and follow the chronological development of editing tools. We explore methodological innovations, including dual pegRNA strategies and site-specific integrases, that have expanded the potential of PE for precise gene insertions. By integrating insights into DNA repair mechanisms and leveraging SpCas9 enhancements, we outline future directions for the application of genome editing in plant breeding.]]></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2025.1719330</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2025.1719330</link>
        <title><![CDATA[Correction: Rewriting the script: gene therapy and genome editing for von Willebrand Disease]]></title>
        <pubdate>2025-11-07T00:00:00Z</pubdate>
        <category>Correction</category>
        <author>Alastair Barraclough</author><author>Isabel Bär</author><author>Tirsa van Duijl</author><author>Karin Fijnvandraat</author><author>Jeroen C. J. Eikenboom</author><author>Frank W. G. Leebeek</author><author>Ruben Bierings</author><author>Jan Voorberg</author><author>Despoina Trasanidou</author>
        <description></description>
      </item><item>
        <guid isPermaLink="true">https://www.frontiersin.org/articles/10.3389/fgeed.2025.1667329</guid>
        <link>https://www.frontiersin.org/articles/10.3389/fgeed.2025.1667329</link>
        <title><![CDATA[Proceedings of the second annual meeting of GenE-HumDi (COST Action 21113)]]></title>
        <pubdate>2025-11-03T00:00:00Z</pubdate>
        <category>Perspective</category>
        <author>María Ortiz-Bueno</author><author>Iris Ramos-Hernández</author><author>Luis Algeciras-Jiménez</author><author>Nechama Kalter</author><author>Juan Roberto Rodríguez-Madoz</author><author>Jose Bonafont</author><author>Rajeevkumar Raveendran Nair</author><author>Oliver Feeney</author><author>Laura Torella</author><author>Lluis Montoliu</author><author>Petros Patsali</author><author>Claudio Mussolino</author><author>Yonglun Luo</author><author>Merita Xhetani</author><author>Alessia Cavazza</author><author>Ayal Hendel</author><author>Karim Benabdellah</author><author>Carsten Werner Lederer</author><author>Francisco J. Molina-Estévez</author>
        <description><![CDATA[Genome editing for the treatment of human disease (GenE-HumDi) is an EU-funded COST Action for the development and consolidation of academic, industrial and healthcare feedback networks aiming to accelerate, foster and harmonize the approval of genome-editing (GE) therapies. GenE-HumDi offers mobility grants, supports educational courses, and hosts conferences and meetings to promote synergistic interactions among and across partners active in the discovery, validation, optimization, manufacturing and clinical application of genomic medicines. Furthermore, it provides young and early career scientists with a supportive and world-class environment to foster networking and international collaborations within the GE field. We compiled the proceedings of the second Annual GenE-HumDi Meeting held in Limassol, Cyprus, in 2024. Over three days, renowned experts from the field updated an audience of over 70 GenE-HumDi members and non-member scientists on the latest discoveries and ongoing projects, discussed the status of the field, and identified GenE-HumDi action priorities to advance research and development for GE medicines. Seven focused discussion groups identified gaps in knowledge, standardization and dissemination for new GE tools, delivery methods, safety monitoring, validation for clinical use, and progress in industrial manufacturing and regulatory issues. Simultaneously, publicity about the event itself contributed to outreach and dissemination of GE for human diseases. Therefore, the conclusions of that meeting, summarized here, serve as a compass toward GE application in Europe through coordination, enhanced collaboration and focus on critical developments.]]></description>
      </item>
      </channel>
    </rss>