The opening keynote set an ambitious tone. Wendy Bickmore, director of the MRC Human Genetics Unit at the University of Edinburgh and a pioneer in functional three-dimensional genome organization, delivered the special EMBO Keynote lecture on how the non-coding genome regulates gene activity. She illustrated that distant enhancers do not always need direct physical contact with their target promoters to activate gene expression, but they must be located within roughly 200 to 300 nanometers of a promoter to function effectively. Bickmore showed that cohesin-mediated loop-extrusion is essential for long-range enhancer action, while also challenging the loop-extrusion model as the sole explanation, presenting evidence from her laboratory of ‘leaky’ insulation across topologically associating domain boundaries that causes bystander activation. She also unveiled a novel histone post-translational modification, H3K115 acetylation, which sits within the histone core rather than on the tail and is enriched precisely at the transcription start site in the nucleosome-depleted region, suggesting it marks a fragile nucleosome strongly associated with active transcription.

On the second day, Lei Stanley Qi, associate professor of bioengineering at Stanford University and a pioneer in CRISPR technology, offered a conceptual reframing of how scientists should interpret chromatin maps. TAD boundaries, he argued, are merely snapshots of chromatin interactions, whereas a cell functions as a living, dynamic system. He drew an evocative parallel with Leonardo da Vinci’s Vitruvian Man, which captures optional configurations of the human body, much as epigenetic figures capture the states of many cells across time and space. Qi described an epistasis mapping approach to enhancer functionality, explaining how redundant, independent, or synergistic enhancer interactions can provide compensatory, fine-tuning, or robust regulatory effects respectively, and noted that BRD4-mediated condensation can facilitate such interactions. Notably, his findings independently confirmed Bickmore’s conclusion that enhancers need spatial proximity to promoters to exert their effects.

The final keynote, from Angelo Lombardo, professor of tissue biology and regenerative medicine at Vita-Salute San Raffaele University and co-founder of Chroma Medicine, delivered perhaps the strongest evidence yet that epigenetic editing can work as a durable therapy. His laboratory discovered that stable gene repression requires simultaneous methylation of DNA and repressive histone marks, and that epigenetic regulators such as DNMT3A/3L and KRAB domains, which catalyze DNA and histone methylation, silence retroviral elements in embryonic stem cells. Inspired by this natural system, the group fused DNMT3A/3L and the KRAB domain of ZNF10 to zinc finger domains targeting specific genomic regions, achieving stable gene repression across multiple cell lines. They recently demonstrated long-term repression of PCSK9, a hepatocyte gene involved in cholesterol homeostasis, in mice for nearly one year, reducing LDL receptor presence on hepatocyte membranes. Strikingly, even after partial liver resection, the induced DNA methylation state and repressed expression were retained in the regrown tissue, showing that these modifications are faithfully inherited. Lombardo also highlighted epigenetic silencing of Hepatitis B virus via induced DNA methylation as a viable therapeutic avenue.

Beyond the keynotes, a wave of technical innovation is reshaping how epigenetic enzymes are understood and improved. Albert Jeltsch of the University of Stuttgart uses Deep Enzymology to systematically investigate the preferred flanking DNA sequences of DNA methyltransferases, finding that different DNA substrates influence DNMT1 efficacy so drastically that allele-specific DNA methylation becomes possible. Saulius Klimašauskas and colleagues at Vilnius University developed a click-chemistry technique for bioorthogonal labeling at sites where individual DNMTs catalyze methylation in live cells, enabling high-resolution chemical ‘tracks’ of epigenetic writers throughout the cell cycle. At Rice University, Jacob Goell reduced the cytotoxicity of the histone acetyltransferase P300 while preserving its enzymatic activity through a single point mutation in the P300 core, and found that P300 primes genes for activation and enhances prime editing efficiency independently of its catalytic function.

Epigenetic reader domains, which evolved over millions of years to recognize specific post-translational modifications, are also becoming central tools, particularly where high-quality antibodies are hard to develop. Tuncay Baubec of Utrecht University presented ChromID, a systematic approach in which a biotin ligase fused to a chromatin reader domain biotinylates nearby proteins; after pull-down and mass spectrometry, the epigenetic proteome at a targeted modification is mapped. EpiCypher’s Matthew Meiners described chimeric tandem reader domains and synthetic, fully chemically defined modified nucleosomes for use as spike-ins in CUT&RUN and CUT&Tag assays, allowing researchers to map reader-PTM interactions and histone modification co-occurrences. Anja Köhler of the University of Stuttgart introduced the Bimolecular Anchor Detector, or BiAD, technology, which combines a sgRNA/dCas9 DNA-binding module with reader-domain detector modules fused to complementary split fluorophore parts, reconstituting fluorescence only when both modules bind in proximity, thereby visualizing epigenetic marks at specific genomic loci in living cells. Meanwhile, Marvin Tanenbaum of the Hubrecht Institute presented stopless-ORF circular mRNAs encoding SunTag epitopes, permitting live-cell single-molecule imaging of ribosome kinetics and revealing that ribosome collisions actually facilitate translation through difficult sequences by resolving stalls.

As the toolbox expands, so does the appetite for unbiased, high-throughput screening. Lacramioara Bintu’s laboratory at Stanford developed dCas9-mediated high-throughput recruitment, or HT-recruit, testing more than 5,000 nuclear protein Pfam domains of human and viral origin for their ability to silence or activate gene expression, alongside a library of 114,288 sequences tiling transcription factors and chromatin regulators. Her characterization was memorably vivid: transcriptional activators tend to be ‘greasy acidic noodles with a little salt, pepper and queso,’ rich in acidic and hydrophobic residues interspersed with serine, proline, or glutamine, while repressors come in more flavors, with KRAB domains the best performers across contexts, including a newly identified KRAB from ZNF705F that outperforms the commonly used ZNF10 KRAB. At UC Berkeley, Michael Herschl screened over 50,000 pairs of epigenetic editors, some with catalytic domains up to 6.3 kilobases, using the COMBINE inducible screening platform, identifying editor combinations that impart long-term epigenetic changes and a bidirectional CRISPR perturbation system capable of activating and repressing genes concurrently. A key insight: domains operating in the same or similar pathways show good perturbation synergy, mimicking their natural collaboration. Samuel Reisman of Duke University, in work toward regenerative therapies, screened over 1,600 human transcription factors with CRISPR activation followed by Perturb-seq single-cell RNA sequencing to map the fidelity and subtype-specificity of astrocyte-to-neuron reprogramming.

Computational advances featured prominently as well. Kim Kira Witetzek of Academia Sinica presented ATAC-Mass, which combines isotopic labeling, ion beam imaging at 100-nanometer resolution, and mass cytometry to integrate epigenomics, proteomics, and three-dimensional nuclear imaging at the single-cell level. Jennifer Spangle of Emory University School of Medicine described a chemoenzymatic technique using an L-methionine analogue that converts into a SAM analogue, tagging methylated proteins with a detectable alkyne; the approach resolves mono-, di-, and trimethylation, histidine methylation, and arginine methylation with site specificity, works in vivo and across the blood-brain barrier, and identified 221 proteins with novel methylation sites upon enrichment. Philipp Schnee of the University of Stuttgart showed how 3D molecular dynamics simulations can predict enzyme behavior, enabling the design of a ‘Super-Substrate’ for protein lysine methyltransferases that outcompetes natural substrates with substantially increased specificity. Kimberley Glass of Brigham and Women’s Hospital presented SPIDER, a computational modeling tool that builds gene regulatory networks from DNase-seq, ATAC-seq, or DNA methylation data, prunes false positives using chromatin states, and accurately predicts ChIP-seq transcription factor binding events lacking a corresponding sequence motif, a persistent weakness of older pipelines.

The field’s clinical momentum was matched by growing candor about its risks. Jamie Hackett of EMBL Rome used CRISPR-dCas9 perturbation screens to dissect causal regulatory roles, finding that blocking histone tail acetylation prevents transcriptional activation after H3K4me3 deposition, and that gene permissiveness to epigenetic reprogramming depends on cell type, expressed factors, and DNA sequence. Domitilla del Vecchio of MIT proposed that H3K9me3 causally follows DNA methylation, noting that KRAB alone does not confer long-term memory while DNMT3A does. Bas van Steensel of the Netherlands Cancer Institute used transposon systems to relocate enhancers, promoters, and CTCF sites across a two-megabase window, discovering that enhancers communicate with gene bodies as well as promoters. On safety, Henriette O’Geen of UC Davis showed that hundreds of CpGs retain off-target methylation 24 days after transient editing, particularly at bivalent genes poised for transcription and implicated in oncogenesis, prompting a call for a gold standard for reporting off-target effects; Majid Pahlevan Kakhki of Karolinska Institutet independently reported widespread unintended methylation across nearly all CRISPR-dCas9 tools, including CRISPRoff. In applied settings, Pernette Verschure’s group found transcription burst size predicts gene responsiveness in hormone-sensitive breast cancer, while Gabriella Ficz of Barts Cancer Institute demonstrated ex vivo epigenetic editing of CDKN2B in umbilical cord hematopoietic stem cells, with durable methylation maintained after engraftment in mice and inherited across myeloid and lymphoid lineages. Ivana Parker of the University of Florida, meanwhile, mapped the epigenetic pathways underlying BCG vaccine-induced macrophage activation. Together, the Amsterdam meeting captured a field in confident transition: from conceptual understanding of chromatin’s static architecture to the dynamic, engineered, and increasingly therapeutic manipulation of the epigenome, balanced by a maturing commitment to safety, standardization, and open collaboration between academia and industry.

Subject of Research: Epigenetic editing technologies and their translation from bioengineering innovations toward clinical therapies

Article Title: Bridging bioengineering and epigenetics: from technical innovations to clinical applications

Article References: Jacob, J., van Loosen, Q. C., van den Berg van Saparoea, A. C. H., Sarno, F., & Verschure, P. J. (2024). Bridging bioengineering and epigenetics: from technical innovations to clinical applications. Epigenetics Communications, 4(1), Article 8. https://doi.org/10.1186/s43682-024-00031-x

Image Credits: AI Generated

DOI: 10.1186/s43682-024-00031-x

Keywords: epigenetics, bioengineering, CRISPR, epigenome editing, DNA methylation, chromatin, gene regulation, clinical applications, off-target effects, high-throughput screening, transcription, gene therapy

Epigenome editing has emerged as a programmable alternative to cutting DNA. Rather than introducing double-strand breaks that can carry risks of unintended mutations and chromosomal rearrangements, epigenetic editors park a catalytically inactive CRISPR protein at a chosen genomic address and ferry enzyme domains that chemically modify histones or DNA, dialing gene expression up or down. The approach holds obvious therapeutic appeal, particularly for diseases in which silencing a gene, an enhancer, or a viral genome could produce lasting benefit. But the most widely used scaffolds, based on the large nuclease-dead Cas9 and Cas12a proteins, are simply too big for the delivery workhorses of gene therapy. Adeno-associated virus vectors, prized for their safety record and tissue tropism, carry only about 4.7 kilobases of genetic payload, and a full epigenetic editor with its guide RNA and effector domains routinely overflows that budget, forcing cumbersome dual-vector strategies that reduce efficiency and complicate manufacturing.

The Peking University team’s solution began with a systematic search of microbial genomes. Through iterative bioinformatic analysis using hidden Markov model profiling and sequence similarity searches, they cataloged miniature Cas12m effectors belonging to CRISPR subtype V-M, with particular attention to homologs that lack the canonical DED catalytic motif required for DNA cleavage. Previous work had established that some Cas12m proteins bind DNA programmably without cutting it, but their utility as epigenome-editing scaffolds remained unproven. Among the candidates, the enzyme from P. methylotrophicum, PmCas12m, stood out. Functional assays showed that it recognizes a flexible 5′-YTN-3′ protospacer-adjacent motif, a permissive target range far broader than many larger editors, and that it grips double-stranded DNA robustly while displaying no detectable DNA cleavage activity in vitro. Those properties, tight binding without cutting, are precisely the profile desired for a protein whose job is to serve as a molecular delivery truck for epigenetic modifiers.

To understand why PmCas12m binds but never slices, the researchers turned to cryo-electron microscopy, solving structures of the protein in complex with its CRISPR RNA and target DNA. The resulting maps, deposited in the Protein Data Bank and the Electron Microscopy Data Bank, reveal the architecture of a compact single-domain effector and trace the network of contacts that PmCas12m makes with the guide RNA, the DNA-RNA hybrid formed upon target recognition, and the displaced non-target strand. The structures explain how the enzyme accommodates its permissive YTN PAM and show that although the RuvC nuclease domain region is present in degraded form, the catalytic machinery needed to position metal ions for phosphodiester cleavage is functionally absent. In other words, PmCas12m is nuclease-dead not by accident of a single mutation but as an innate, evolutionarily entrenched property, a feature that removes the need for artificial inactivation and the performance penalties that often accompany it.

Structural insight then became a design tool. Guided by the cryo-EM maps, the team examined which parts of the protein were dispensable and which residues constrained or enabled function, and they applied deep mutational scanning, a technique that simultaneously tests the effects of thousands of amino acid substitutions, to map the protein’s tolerance landscape. Iterative rounds of rational deletion and mutation, informed by both the experimental scan and computational structure predictions, yielded xCas12m, a hypercompact variant that retains specific DNA recognition while acquiring highly potent epigenome-editing capability in human cells. The engineering strategy mirrors approaches that have successfully miniaturized other compact editors, such as Cas12f and IscB, but here it was applied to a protein that needed no catalytic rescue, only optimization of binding, expression, and compatibility with effector fusions.

With the scaffold in hand, the researchers built xCas12m-CRISPRoff, a silencing platform in which the miniature protein is fused to repressive chromatin-modifying domains of the kind used in canonical CRISPRoff systems, including KRAB repressor domains and methyl-CpG-binding protein modules. Tethered to gene promoters by single guide RNAs, the system laid down repressive epigenetic marks that persisted after the editing machinery itself was no longer detectably active, reproducing the durable, heritable transcriptional memory that makes CRISPRoff-style tools attractive for both research and therapy. The team also demonstrated the converse capability, showing that xCas12m fused to activation domains such as VPR could drive expression of endogenous genes in human cells, confirming that the miniature scaffold is a versatile platform for bidirectional control of transcription rather than a silencing-only tool.

The delivery advantage then became the centerpiece. Because xCas12m is so small, the entire xCas12m-CRISPRoff system, including the protein, its guide RNA expression cassette, and the necessary regulatory elements, fit within the packaging capacity of a single AAV vector. In a mouse model harboring hepatitis B virus covalently closed circular DNA, the persistent form of the viral genome that current antiviral drugs rarely eliminate, a single administration of the AAV-delivered editor produced durable epigenetic silencing of viral sequences. In treated animals, the researchers measured reduced levels of viral RNA, including pregenomic RNA, and diminished expression of viral antigens, indicating effective inhibition of hepatitis B virus infection through an approach that reprograms the chromatin state of the viral genome rather than cutting it. Because silencing leaves the viral DNA physically intact, the strategy could, in principle, be reversible or tunable, a safety profile distinct from nuclease-based antiviral editors.

The hepatitis B results carry particular weight because chronic HBV infection remains one of the world’s most consequential viral diseases, affecting hundreds of millions of people and driving cirrhosis and liver cancer. Existing therapies suppress replication but seldom achieve a functional cure, largely because the cccDNA reservoir and integrated viral DNA persist in hepatocytes. CRISPR nucleases have been explored as a means to excise or disrupt viral DNA, but they raise concerns about off-target cuts in the human genome and about delivery, since Cas9-based antiviral systems typically strain or exceed AAV capacity. An epigenetic editor that arrives in one viral particle, targets the viral genome with programmable guides, and extinguishes its transcription without touching the host sequence offers a conceptually different route toward functional cure, one that the authors position as a step toward clinical translation of epigenetic therapies.

Cautions remain before such promises can be evaluated in patients. Off-target DNA binding by any guide-directed protein must be mapped comprehensively across the genome, the durability and stability of the silenced state must be tracked over long periods, and immune responses to a bacterial protein delivered by AAV in the liver will need careful assessment. The specificity data reported for xCas12m in human cells are encouraging, and the compact size may itself reduce immunogenic surfaces, but these questions will only be settled in larger animal models and, eventually, carefully designed trials. What the study establishes now is a proof of principle that structure-guided discovery plus deep mutational scanning can compress an epigenome editor into a single-vector package without sacrificing potency. In doing so, it hands the field a new miniature chassis, xCas12m, that could carry epigenetic payloads to targets previously out of reach, from repressing disease genes to quieting persistent viral genomes, and it demonstrates how atomic-level structural biology continues to reshape what therapeutic genome engineering can look like.

Subject of Research: Structure-guided discovery and engineering of the miniature nuclease-dead CRISPR–Cas12m protein for AAV-deliverable epigenome editing and hepatitis B virus silencing

Article Title: Structure-guided discovery and engineering of miniature CRISPR–Cas12m for epigenome editing

Article References: Yu, T., Ji, M., Yu, D., Guan, Z., Zhu, R., Jiang, Y., Yang, Z., Qiu, L., Zhang, Z., Mu, J., Mao, F., Xiang, K., Bai, L., & Li, K. (2026). Structure-guided discovery and engineering of miniature CRISPR–Cas12m for epigenome editing. Nature Structural & Molecular Biology. https://doi.org/10.1038/s41594-026-01890-9

Image Credits: AI Generated

DOI: 10.1038/s41594-026-01890-9

Keywords: CRISPR, Cas12m, xCas12m, epigenome editing, CRISPRoff, AAV delivery, gene silencing, hepatitis B virus, cryo-electron microscopy, deep mutational scanning, PmCas12m, gene therapy

The scale of methylation disruption in cancer is staggering. Tumor genomes characteristically display widespread global hypomethylation, in which vast stretches of normally methylated DNA lose their marks, accompanied by focal hypermethylation concentrated at key regulatory regions, particularly the CpG-rich promoters of tumor suppressor genes. The result is an extensive rewiring of gene regulatory networks: genes that restrain cell division are switched off, repetitive elements that are normally locked down become active, and the carefully orchestrated patterns that define cell identity dissolve into chaos. These alterations are so consistent that methylation signatures now underpin diagnostic and prognostic assays used in clinics worldwide, helping pathologists classify tumors, predict patient outcomes, and even trace the tissue of origin of metastatic cancers.

Yet a profound gap separates correlation from causation. The overwhelming majority of cancer-associated methylation changes have never been proven to drive tumor behavior; they may instead be passive consequences of the transformed state. Distinguishing driver marks from passenger marks using observational methylome profiling alone has proved remarkably difficult, because the epigenome is dynamic and context-dependent. This ambiguity has real consequences for drug development. Conventional hypomethylating agents, such as nucleoside analogs that trap and deplete methyltransferase enzymes, can partially reverse cancer-associated methylation alterations and have demonstrated clinical efficacy in selected hematological malignancies. But these drugs act genome-wide, with no capacity to target a specific promoter or enhancer. Their blunt mechanism limits both mechanistic insight—since any observed effect could stem from thousands of altered loci—and therapeutic precision, since desirable and undesirable demethylation occur simultaneously across the genome.

CRISPR-based epigenome editing offers a fundamentally different approach. Rather than cutting DNA, these systems repurpose catalytically inactive Cas proteins, most famously dCas9, as programmable delivery vehicles. Guided to a chosen genomic address by a complementary guide RNA, dCas9 can be fused to methylation ‘writers’—enzymes such as DNMT3A and DNMT3L that install methyl marks—or methylation ‘erasers’, including TET1 catalytic domains and engineered demethylases that oxidize and remove them. Because the underlying DNA sequence is left untouched, the editing is, in principle, reversible, mirroring the reversible nature of the epigenetic alterations themselves. The result is a technology capable of quantitatively tuning methylation at individual promoters, enhancers, and CpG shores—transition zones flanking CpG islands that are frequent sites of cancer-associated methylation gain.

The experimental power of this approach lies in its precision. A single tumor suppressor promoter can be hypermethylated in a controlled setting to test whether silencing of that gene is sufficient to confer growth advantages, or demethylated to ask whether restoring its expression suppresses malignant behavior. Similar logic applies to enhancers, whose methylation status can govern the activity of oncogenes and immune-modulatory genes alike. By editing specific loci, researchers can interrogate mechanisms of chemoresistance, asking whether methylation changes at particular drug-response genes cause treatment failure or merely accompany it. They can also probe immune modulation, since methylation patterns influence the expression of antigen-presenting molecules and immune checkpoint pathways that determine whether tumors are recognized by the immune system. In this way, methylation editing transforms the epigenome from a readout of tumor state into an experimentally addressable variable.

The review also highlights the modular nature of modern CRISPR recruitment platforms, which extend the technology well beyond simple enzyme fusions. Systems such as SunTag, MS2-based scaffolds, and related multiplexing strategies allow multiple effector domains to be recruited to a single target site, amplifying the magnitude of methylation change or combining writers and erasers with transcriptional activators and repressors. Such platforms enable graduated, quantitative manipulation of methylation levels rather than all-or-nothing switching, which is critical because the relationship between methylation density and gene expression is often dose-dependent. Combined with single-cell and multi-omics readouts, these tools allow researchers to observe how a targeted methylation edit propagates through chromatin state, transcription, and ultimately cellular phenotype in diverse cancer models, from cell lines to patient-derived organoids.

None of this progress comes without caveats, and the authors are candid about the obstacles that stand between bench and bedside. Off-target activity remains a central concern: both the DNA-binding specificity of guide RNAs and the promiscuity of the tethered enzymes can produce unintended methylation changes at sites resembling the intended target, and even at sites tethered transiently by direct enzyme-to-dCas9 fusions. Because methylation changes can be heritable through cell division, a single off-target event could have lasting consequences. Context-dependency poses a further complication. The same edit can yield different outcomes depending on chromatin context, cell type, CpG density, and the developmental or disease state of the cell, complicating efforts to generalize results across models. Delivery and durability add clinical dimensions to these challenges: getting large editing constructs efficiently into tumor cells—whether in culture or in a patient—and ensuring that the methylation change persists long enough to be therapeutically meaningful remain unsolved engineering problems.

The path forward, the review argues, lies in integration. Locus-specific editing is poised to converge with comprehensive multi-omics profiling, in which methylome, transcriptome, chromatin accessibility, and three-dimensional genome architecture are measured simultaneously before and after an edit. Machine-learning-guided target selection promises to accelerate this process, mining large epigenomic datasets to prioritize the methylation changes most likely to act as drivers, and to predict how editing a given locus will ripple through regulatory networks. Rational combination therapies represent the clinical endpoint of this vision: methylation editing might, for instance, be paired with immune checkpoint inhibitors by demethylating and reactivating antigen presentation genes, or with conventional chemotherapy by erasing methylation marks that drive drug resistance. Each of these strategies depends on the causal knowledge that only targeted editing can generate.

The significance of this synthesis extends beyond the technical details. For a generation, epigenetic therapy has been constrained by an uncomfortable irony: doctors could alter the cancer epigenome, but only in a coarse, genome-wide fashion that revealed little about which alterations mattered. CRISPR-based methylation editing inverts that logic, making the epigenome writable at single-locus resolution and thereby testable in a way no previous technology allowed. If the challenges of specificity, delivery, and context can be met, the result would be a new class of therapeutics that silence oncogenes or resurrect tumor suppressors without touching a single base of DNA sequence. For now, the technology’s greatest value is as an engine of discovery—a way to finally separate the drivers from the passengers in the cancer methylome. But the trajectory is clear, and the authors’ message is that rewriting the cancer epigenome has moved from metaphor to laboratory reality, with clinical translation as the next horizon.

One reason methylation is such an attractive target for editing is its intrinsic stability. Unlike histone modifications, which turn over rapidly and often require continuous reinforcement, DNA methylation at CpG sites can be faithfully copied through cell division by maintenance methyltransferases that recognize hemimethylated DNA after replication. This means a single, well-placed edit has the potential to persist across many generations of cells, a property that is both a strength for durable therapy and a liability if the wrong loci are modified. The review’s emphasis on precision reflects this double-edged character of the methylation mark.

The choice of effector enzymes also matters greatly. DNMT3A, one of the writer domains commonly fused to dCas9, is itself a gene frequently mutated in hematological malignancies, illustrating how the machinery of methylation regulation is intimately entangled with cancer biology. On the eraser side, catalytic domains derived from the TET enzymes, which normally initiate active demethylation through oxidation of 5-methylcytosine, can be repurposed for targeted removal of marks. That these same pathways are dysregulated in tumors underscores why locus-specific manipulation is such a valuable experimental tool: it allows individual components of an altered network to be tested in isolation.

The work emerges from a research group with a sustained focus on cancer epigenomics at the University of Otago’s Department of Pathology and Molecular Medicine, and the article is published open access under a Creative Commons Attribution license, supported by New Zealand funding bodies including the Health Research Council and the Marsden Fund. Open availability is significant for a methods-oriented review, since widespread adoption of these editing approaches depends on researchers across disciplines and resource settings being able to evaluate the technical trade-offs in detail.

It is also worth noting that the review appears at a moment when epigenome editing more broadly is maturing beyond proof-of-principle demonstrations. The same dCas9 recruitment logic underlies efforts to edit histone marks, chromatin architecture, and transcriptional states, suggesting that methylation editing will ultimately function as one module within a larger toolkit for writing and rewriting the regulatory layer of the genome.

Subject of Research: CRISPR-based DNA methylation editing technologies for interrogating and potentially treating aberrant cancer epigenomes

Article Title: Rewriting the cancer epigenome: CRISPR technologies for DNA methylation editing

Article References: Sadeghi, N., Rodger, E. J., & Chatterjee, A. (2026). Rewriting the cancer epigenome: CRISPR technologies for DNA methylation editing. Cellular and Molecular Life Sciences. https://doi.org/10.1007/s00018-026-06429-1

Image Credits: AI Generated

DOI: 10.1007/s00018-026-06429-1

Keywords: cancer, epigenetics, DNA methylation, CRISPR, DNA methylation editing, dCas9, epigenome editing, tumor suppressor genes, off-target effects, epigenetic therapy, gene regulation, precision medicine