Skip to main content

Peripheral blood DNA methylation and neuroanatomical responses to HDACi treatment that rescues neurological deficits in a Kabuki syndrome mouse model



Recent findings from studies of mouse models of Mendelian disorders of epigenetic machinery strongly support the potential for postnatal therapies to improve neurobehavioral and cognitive deficits. As several of these therapies move into human clinical trials, the search for biomarkers of treatment efficacy is a priority. A potential postnatal treatment of Kabuki syndrome type 1 (KS1), caused by pathogenic variants in KMT2D encoding a histone-lysine methyltransferase, has emerged using a mouse model of KS1 (Kmt2d+/βGeo). In this mouse model, hippocampal memory deficits are ameliorated following treatment with the histone deacetylase inhibitor (HDACi), AR-42. Here, we investigate the effect of both Kmt2d+/βGeo genotype and AR-42 treatment on neuroanatomy and on DNA methylation (DNAm) in peripheral blood. While peripheral blood may not be considered a “primary tissue” with respect to understanding the pathophysiology of neurodevelopmental disorders, it has the potential to serve as an accessible biomarker of disease- and treatment-related changes in the brain.


Half of the KS1 and wildtype mice were treated with 14 days of AR-42. Following treatment, fixed brain samples were imaged using MRI to calculate regional volumes. Blood was assayed for genome-wide DNAm at over 285,000 CpG sites using the Illumina Infinium Mouse Methylation array. DNAm patterns and brain volumes were analyzed in the four groups of animals: wildtype untreated, wildtype AR-42 treated, KS1 untreated and KS1 AR-42 treated.


We defined a DNAm signature in the blood of KS1 mice, that overlapped with the human KS1 DNAm signature. We also found a striking 10% decrease in total brain volume in untreated KS1 mice compared to untreated wildtype, which correlated with DNAm levels in a subset KS1 signature sites, suggesting that disease severity may be reflected in blood DNAm. Treatment with AR-42 ameliorated DNAm aberrations in KS1 mice at a small number of signature sites.


As this treatment impacts both neurological deficits and blood DNAm in mice, future KS clinical trials in humans could be used to assess blood DNAm as an early biomarker of therapeutic efficacy.


Kabuki syndrome type 1 (KS1) is a Mendelian disorder of epigenetic machinery (MDEM) that results from pathogenic variants in KMT2D, a gene encoding a histone H3 lysine 4 (H3K4) methyltransferase [1, 2]. This disorder is characterized by a common set of dysmorphic facial features (e.g., long palpebral fissures with eversion of the lateral third of the lower eyelid; arched and broad eyebrows; short columella), mild-to-moderate intellectual disability, and postnatal growth deficiency. KS1 is also associated with congenital heart defects, increased susceptibility to infections, seizures, and feeding problems [2, 3]. To manage health problems associated with KS1, individuals are followed closely from birth by health care providers to monitor for possible problems or complications and are treated after symptoms arise. Until recently, the idea of an effective postnatal treatment for neurodevelopmental disorders to pre-empt symptoms including developmental delay and intellectual disabilities in disorders such as KS1 seemed highly implausible or at least, remote.

Animal models of KS1 have not only allowed for a deeper understanding of pathophysiology but also provided foundational evidence for effective postnatal treatment of intellectual disability. Bjornsson et al. previously characterized a mouse model of KS1, Kmt2d+/βGeo, for which multiple treatments with drugs with epigenetic modes of action were effective in ameliorating neurological phenotypes. This mouse model recapitulates multiple features of KS1 including facial dysmorphism, learning deficits, immune dysregulation and has been characterized as exhibiting global loss of histone H3K4 trimethylation (H3K4me3) in vitro and in vivo [4,5,6] and aberrant chromatin accessibility [7]. AR-42, a histone deacetylase inhibitor (HDACi), improved hippocampal learning and memory deficits in Kmt2d+/βGeo mice, as well as normalized H3K4me3 levels in the dentate gyrus [4]. Inhibition of KDM1A using TAK-418, a histone demethylase that removes H3K4 methylation, or increasing endogenous HDACi beta-hydroxybutyrate through a ketogenic diet led to similar phenotypic rescues in this mouse model [5, 6]. These findings have precipitated clinical trials of dietary interventions as a treatment for cognitive deficits in individuals with KS1 (Identifier NCT04722315).

In many MDEM, DNA methylation (DNAm) has proven to be an effective diagnostic tool in the research and clinical settings [8,9,10,11]. Our group published a DNAm signature of KS1 in 2017, finding this pattern of methylation to be distinct from CHARGE syndrome (a differential diagnosis) but not Kabuki type 2, caused by pathogenic variants in the X-linked gene KDM6A [12]. Other KS signatures have also been defined, demonstrating similar findings with specificity for the KS phenotype [13, 14]. Both KMT2D and KDM6A act to promote open chromatin by depositing activating H3K4me or removing repressive H3K27me2/3, respectively [15,16,17]. The human KS1 signature currently serves multiple functions including classifying variants of uncertain significance as pathogenic or benign and providing a set of loci at which transcriptional dysregulation may be contributing to the KS1 phenotype and severity [12, 13, 18]. However, there may be even greater potential for DNAm signatures as it is possible that these may work as a therapeutic biomarker capturing information of sub-phenotype presence/absence and treatment efficacy. In drug trials of treatments for neurological outcomes, biomarkers raise the success of these trials from 11 to 40% [19].

Here, we establish a KS1 mouse signature in blood DNA and assess whether this signature can serve as a biomarker of (1) phenotypic severity as measured by brain volume, and (2) treatment efficacy of AR-42. We find that the KS1 mouse signature maps to genes that exhibit DNAm aberrations in humans with KS1. Additionally, a subset of signature sites are predictive of brain volume, while a different subset exhibits a correction of DNAm levels in the AR-42 treated KS1 mice, i.e., a shift toward normal wildtype (WT) DNAm levels. Moreover, previously published H3K4me3 levels primarily showed unidirectional changes, with genome-wide loss of H3K4me3 in the Kmt2d+/βGeo mice and genome-wide gain of H3K4me3 in response to AR-42 treatment [4]. Our corresponding DNAm data exhibited bidirectional changes, with no bias toward gain or loss of methylation with this genotype or following AR-42 treatment. While a simplified model of epigenetic cross-talk may predict gain of H3K4me3 to correspond to a loss of DNAm and vice versa, we saw no such relationship, highlighting the complexity of epigenetic regulation and downstream effects of disruption of transcriptional programs resultant from epigenetic perturbations. This work supports a new area of exploration for DNAm signatures, as biomarkers of treatment efficacy.



Methods for treatment with AR-42 follow those published in Bjornsson et al. [4]. Briefly, the KS1 mouse model, Kmt2d+/βGeo was acquired from Bay Genomics (University of California) but have since been fully backcrossed onto a pure C57BL/6J background. Mice were housed at the Johns Hopkins Mouse Facility. Animals in this study were born across 9 litters resulted from timed matings within a 3–4 day window, and assorted in genotype and sex matched pairs to cage, and treatment group. Only males were used in this experiment in an effort to provide sex-disaggregated data while also being limited by experimental time and cost constraints. Mice were dosed by oral gavage daily beginning at postnatal week 4 for 2 weeks, with vehicle alone (0.5% methylcellulose, 0.1% Tween-80, water) or treated with vehicle + 10mg/kg AR-42 (Selleck Chemicals). Cages were randomly selected for sacrifice one or two days after the end of treatment. Mice were weighed and blood was collected from the submandibular vein into K2EDTA-coated microtainer tubes (lavender top) for epigenetic analysis. Mice were anesthetized with a lethal dose of ketamine/xylazine and prepared by transcardiac perfusion (first flush: PBS + 1USP/mL heparin + 2mM ProHance, second flush: 4%PFA + 2mM ProHance), and skulls were stored in 4% PFA + 2mM ProHance overnight. Buffer was replaced with 1xPBS + 0.02% sodium azide + 2mM ProHance and stored 4C until imaging. As all samples did not meet quality control, experiments differ in their sample sizes despite being run on “matched” tissues (Table 1). All experiments were performed using mouse protocols approved by the Animal Care and Use Committee of Johns Hopkins University School of Medicine (Baltimore, USA) and the Animal Care Committee of The Centre for Phenogenomics (Toronto, Canada). The mouse protocols used for this study are in accordance with the guidelines used by the National Institutes of Health (NIH) for mouse care and handling and the Canadian Council on Animal Care (CCAC).

Table 1 Sample sizes

DNA extraction

DNA was extracted from mouse blood stored at − 80 °C, using phenol–chloroform method. This was then repeated to purify DNA. PCR was run on genomic DNA using primers B-GeoF-(CAAATGGCGAT-TACCGTTGA) and B-GeoR-(TGCCCAGTCATAGCCGAATA), which are specific for the targeted allele to confirm genotype. Genomic DNA was then bisulfite converted using the EpiTect Bisulfite Kit (EpiTect PLUSBisulfite Kit, QIAGEN).

DNA methylation microarray and statistical analysis

DNAm was assayed using the Illumina Infinium Mouse Methylation BeadChip (> 285,000 CpG sites) at The Center for Applied Genomics (TCAG), Hospital for Sick Children Research Institute, Toronto, Ontario, Canada in accordance with the manufacturer’s protocols. Samples were randomized on to array chips such that chips were balanced for genotype and treatment.

Mouse array data were background corrected and normalized in Genome Studio using Illumina normalization and then imported into R for further data preprocessing and analysis. CpG sites with a detection p-value greater than 0.05 were replaced with N/A, as well as sites covered by less than three beads. Probes mapping to mitochondrial DNA were also removed, but sex chromosomes probes were left in as all mice were male. A total of 284,394 CpGs remained following data cleaning.

Three outliers were identified by the detectOutlier function in the lumi package and were removed leaving a total of 40 samples for analysis: n = 13 vehicle-treated wildtype (vehicle WT), n = 8 AR-42-treated wildtype (AR-42 WT), n = 10 vehicle-treated Kmt2d+/βGeo (vehicle Kmt2d+/βGeo), n = 9 AR-42-treated Kmt2d+/βGeo (AR-42 Kmt2d+/βGeo) [20].

CpG sites differentially methylated by genotype, treatment, or phenotypic measures were identified using Limma regression, a modified linear regression run on log transformed beta values, M values [21, 22]. As blood is composed of multiple cell types with unique identities and therefore methylation patterns, 2 surrogate variables were included as covariates to account for major sources of underlying inter-individual variation [23, 24]. The number of significant SVs was determined by the “” function, using the Leek method and a model that included genotype or treatment, depending on which samples would be included in the model, and day of sacrifice [25]. SVs were generated using only the samples used in any given analysis. SVs were not included as covariates in the model in which total brain volume predicted DNAm. Day of sacrifice, i.e., 1 or 2 days following treatment, was also included as a covariate. Litter was excluded as there were no observable trends in DNAm between litters, as estimated by principal component 1 and 2 (PCs generated on all CpGs used in analysis; Additional file 1: Figure S1). CpGs reported as significant met genome-wide significance following False Discovery Rate (FDR) correction (q-value < 0.05) and a minimum effect size of mean group methylation difference above 5% (delta beta > 5%). For certain analyses, the q-value was relaxed to less than 0.1 as stated in text.

Differentially methylated regions (DMRs) were identified using combp function from the package ENmix [26]. Raw p-values from limma and CpG coordinates were fed into combp to identify regions at which p-values were measurably lower than surrounding sites. The FDR significance threshold for DMR identification was set to < 0.005. After DMRs were identified, they were manually subset to those containing at least 3 CpGs all with hypo- or hypermethylation, or at least 3 CpGs with hypo- or hypermethylation (if DMR contained more three CpGs and had bidirectional methylation changes). As well, each DMR had to contain at least one CpG found significant in the limma analysis.

Brain imaging

Fixed brain samples were imaged using MRI to calculate regional volume [27]. A multi-channel 7.0 Tesla MRI scanner (Agilent Inc., Palo Alto, CA) was used to image the brains within their skulls. Sixteen custom-built solenoid coils were used to image the brains in parallel [28]. In order to detect volumetric changes, we used the following parameters for the MRI scan: T2- weighted, 3-D fast spin-echo sequence, with a cylindrical acquisition of k-space, a TR of 350 ms, and TEs of 12 ms per echo for 6 echoes, field-of-view equaled to 20 × 20 × 25 mm3 and matrix size equaled to 504 × 504 × 630. Our parameters output an image with 0.040 mm isotropic voxels. The total imaging time was 14 h [29].

MRI registration and analysis

To visualize and compare any changes in the mouse brains the images are linearly (6 followed by 12 parameter) and nonlinearly registered together. Registrations are performed with a combination of mni_autoreg tools and ANTS (advanced normalization tools) [30,31,32]. In this process, scans are resampled with the appropriate transform and averaged to create a consensus population atlas representing the average anatomy of all brains. The result of the registration is to have all images deformed into alignment with each other in an unbiased fashion. This allows for the analysis of the deformations needed to take each individual mouse's anatomy into this final atlas space, with the ultimate goal being to model how the deformation fields relate to genotype [33, 34]. For a voxelwise analysis, the jacobian determinants of the deformation fields are calculated as measures of volume at each voxel. Regional differences can be calculated by warping a pre-existing classified MRI atlas onto the population atlas, which allows for the volume of 282 different segmented structures encompassing cortical lobes, large white matter structures (i.e., corpus callosum), ventricles, cerebellum, brain stem, and olfactory bulbs to be assessed in all brains [35,36,37]. Multiple comparisons in this study were controlled for using FDR [38].


Kmt2d +/βGeo mouse brain volume and body weight

Kmt2d+/βGeo mice, carry an expression cassette encoding a β-galactosidase neomycin resistance fusion protein (β-Geo) in intron 50 of Kmt2d [4]. This allele produces a truncated protein that is lacking the SET domain, which confers methyltransferase activity to this protein. Forty-seven mice were born as 9 litters and assorted in sex and genotype matched pairs to minimize cage effects. Mice were weighed prior to sacrifice, at 6 weeks, and Kmt2d+/βGeo mice (vehicle-treated; n = 10) were found to be significantly smaller than WT (vehicle-treated; n = 13; Fig. 1a). Growth retardation compared to WT littermates has previously been described in Kmt2d+/βGeo mice at 5 months [4]. Of note, individuals with KS1 tend to have normal birth parameters but often exhibit failure to thrive and postnatal growth deficiency, in part due to feeding and gastrointestinal problems [3].

Fig. 1
figure 1

Size and brain volume deficits in Kmt2d+/βGeo mice. A Body weights (g) of vehicle-treated animals at sacrifice. Kmt2d+/βGeo animals were significantly smaller than WT (t-test p-value < 0.05). B Absolute (left) and relative (right) volume changes in Kmt2d+/βGeo for all structures with q-value < 0.05. As observed in left column, volume loss is consistent across brain structures. C Total brain volume (mm3) vehicle-treated animals. Kmt2d+/βGeo volumes were significantly smaller than WT (t-test p-value < 0.05)

In additional to Kmt2d+/βGeo mice having lower body weight, they exhibited significantly lower total brain volume at 6 weeks, as compared to WT (vehicle-treated groups; n = 9 Kmt2d+/βGeo and n = 11 WT; q-value < 0.001; Fig. 1b). While total brain volume was decreased by 10% in the Kmt2d+/βGeo group, specific regions with the largest differences include white matter (− 12.7%, q < 0.001), isocortex (− 12.4%, q < 0.001, and the olfactory areas (-11.3%, q < 0.01). As expected, brain volume was strongly correlated with body weight at sacrifice (Additional file 1: Figure S2). When relative volume was measured (regions as a percentage of total brain volume), the significance of some of these large areas was lost. However, more specific differences remained, including a relative volume decrease in the corpus callosum (− 5.4%, q = 0.01), and a relative increase in striatum (+ 7.25%, q = 0 < 0.001), the hypothalamus (+ 7.1%, q = 0.001), and the deep cerebellar nuclei (+ 3.3%, q = 0.04). There also was a trend found for a relative volume decrease in the overall isocortex (− 2.5% q = 0.07), indicating a larger cortical decrease comparatively to the whole brain volume. The hippocampus has previously been implicated in neurological phenotype of this mouse model and was found to be smaller in individuals with KS [4, 6, 39]; here, we found the hippocampal region and all underlying structures to have significantly smaller absolute volumes in Kmt2d+/βGeo mice (q < 0.05). The hippocampal region and dentate gyrus showed volume differences of − 9.9% and − 11.4%, respectively. When relative volumes were taken into account hippocampal differences were localized to the stratum radiatum of CA1. Please see Additional file 2: Table S1 for a list of all structures investigated and corresponding p-values.

Kabuki mouse DNA methylation signature overlaps with human KS1 signature and is enriched for genes with neurological functions

We compared the vehicle treated animals, Kmt2d+/βGeo (n = 13) versus WT littermates (n = 10), to identify CpG sites differentially methylated by genotype. A linear model was applied to all CpGs sites on the array that passed quality control; 1599 CpGs met significance (q-value < 0.05; delta beta > 5%; Fig. 2a; Additional file 1: Figure S3; Additional file 2: Table S2), with 769 CpGs (48%) exhibiting hypermethylation in the Kmt2d+/βGeo group, as compared to WT (Fig. 2b). This set of CpGs, hereafter referred to as a KS1 mouse “signature”, was tested for robustness using leave-one-out cross validation. The methylation patterns demonstrated 100% specificity and sensitivity, with all samples correctly predicted as WT or KS1 when validated on a signature generated on remaining samples (Fig. 2c).

Fig. 2
figure 2

KS1 mouse signature has high sensitivity and specificity, as determined by cross-validation. A PCA at 1599 signature sites in only vehicle-treated samples (n = 13 WT; n = 10 KS1). B Heatmap of signature sites, showing even split between hyper- and hypomethylation, as well as clustering of samples by genotype. Dendrograms generated with Euclidean clustering. DNA methylation (Beta values) is normalized and ranges from − 2 to 2  C Leave-one-out cross-validation shows all samples correctly clustering by genotype. Samples, when left out and used for cross-validation, are more strongly correlated with samples of the genotype at signature sites

Signature sites were also assessed for a difference in variances between genotypes as Kmt2d+/βGeo mice may exhibit a general loss of control or dysregulation of DNAm patterns in addition to a directional shift in methylation. 73% of signature sites (1173) exhibited a larger range in the Kmt2d+/βGeo group, as compared to WT; however, this difference was only found to be significant in one CpG, which mapped to the gene body of Ndst1 (cg35789886_BC11; Levene’s test q < 0.05; Additional file 2: Table S2).

GO enrichment analysis was applied to signature sites, both hyper- and hypomethylated in KS1 mice, and significant cell component terms (q-value < 0.01) were specific to neuronal cells and included dendrite, post synapse and axon, while common biological process terms and molecular function terms included those related to cell morphogenesis and kinase activity, respectively (Fig. 3a and b; Additional file 1: Figure S4). We also compared signature sites to loci previously implicated in KS1, either in humans or in the KS1 mouse model presented here. Butcher et al. [12] published a blood KS1 signature on 11 individuals with KS1, which contained 221 CpG sites [12]. Nineteen genes were found to map to differential methylation in both the human and mouse signature (Table 2). Of those 19 genes, 15 genes exhibited methylation changes in the same direction in KS1 samples. A number of genes had described functions in neuronal tissue or were associated with autosomal dominant phenotypes in humans with neurodevelopmental or neurological features, including SLITRK5, DLG4, ZMIZ1, RA1 and VAC14. Differential expression analysis was performed on Kmt2d+/βGeo and WT littermates’ hippocampal cells and published in Zhang et al. [6]. There were 345 differentially expressed transcripts that met a q-value < 0.15, which mapped to 77 unique genes [6]. Five genes were found to be differentially expressed in Kmt2d+/βGeo hippocampi and differentially methylated in Kmt2d+/βGeo blood: Ddx39b, Jarid2, Prph, Tyro3, Snhg1.

Fig. 3
figure 3

KS1 mouse signature sites mapped to genes related to KS1 phenotype. A GO enrichment top ten enriched cell component terms are specific to neuronal cells. B GO enrichment top ten enriched biological process terms are specific to neuronal cells. C DMR in the last exon of transcription factor MYC, composed of 5 CpGs, and overlaps proximal- and distal-acting enhancers

Table 2 Overlapping differential methylation in mouse and human KS1 signatures

Finally, using the same set of vehicle-treated samples, we identified 99 differentially methylated regions (DMRs), each containing least three CpGs and at least one signature CpG (Additional file 1: Table S3). Similar to the direction of change observed in the signature, DMRs were evenly split between those containing hyper- vs. hypomethylated sites; specifically, 48 DMRs contained all hypermethylated CpGs; 49 DMRs contained all hypomethylated CpGs; and 2 DMRs contain CpGs with bidirectional changes. Multiple DMRs mapped to genes with functions that may relate to KS1 pathophysiology; these included the transcription factor Myc (Fig. 3c); protocadherin Pcdh7; GABA type B receptor Gabbr2; interferon regulatory factor Irf6; and synaptic vesicle glycoprotein Sv2c. As well, one DMR was intronic to Jarid2, which is differentially expressed in Kmt2d+/βGeo hippocampi and one DMR mapped to Slitrk2, encoding a membrane protein expressed predominantly in neural tissue, which is differentially methylated in the blood of individuals with KS1.

Kabuki mouse DNA methylation signature sites predict brain volume

We analyzed the vehicle-treated animals, Kmt2d+/βGeo and WT, for a relationship between total brain volume and DNAm. Starting with the 1599 signature CpGs, we ran a model in which total brain volume was treated as the main effect and identified 27 significant CpGs (q-value < 0.05, delta beta > 5%; Additional file 1: Figure S5; Additional file 2: Table S4). A principal component analysis applied to these 27 CpGs revealed a clearer trend between DNAm and brain volume in the Kmt2d+/βGeo mice, as compared to the WT, although this relationship did not meet statistical significance within either genotype (WT p-value < 0.66; Kmt2d+/βGeo p-value = 0.13; Fig. 4). Nonetheless, the F-statistic in Kmt2d+/βGeo mice was 3.04, as compared to 0.21 in WT mice, indicating a trend between these blood DNAm patterns and brain volume that may meet significance with a larger sample size. This difference in the strength of the association between Kmt2d+/βGeo mice and WT, may be related to the differing ranges of brain volumes between genotypes, i.e., across WT animals, there is a range of ~ 40mm3 in total brain volume (min. 402.7; max. 442.5; median 425.4), and across Kmt2d+/βGeo animals, there is a range of ~ 90mm3 in total brain volume (min. 327.5; max. 417.9; median 388.7). Alternatively, this relationship between DNAm and brain volume may be specific to or stronger in Kmt2d+/βGeo mice and a consequence of epigenetic dysregulation. Supporting this scenario, the animals most severely affected are seen to have both the smallest brain volumes and greatest changes in methylation levels.

Fig. 4
figure 4

Linear relationship between brain volume and DNAm level at 27 CpGs in Kmt2d+/βGe mice (left), as compared to WT mice (right). Y-axis represents PC1 scores of each animal, derived from PCA of 27 signature CpGs significantly associated with total brain volume. Blue lines represent line of best fit and statistics were generated from a linear regression performed within each group

Effects of AR-42 treatment on brain volume and blood DNA methylation

Next, we compared the vehicle- and AR-42-treated Kmt2d+/βGeo animals to identify any changes to methylation patterns and/or brain volume. AR-42-treated Kmt2d+/βGeo did not significantly differ from vehicle-treated Kmt2d+/βGeo in brain volume (all structures q value > 0.05, data not shown). For WT mice only, the effect of treatment appeared to have a marginal trend toward a decrease in size (− 3.4%, p < 0.03, q < 0.16). However, this same trend was not seen in the Kmt2d+/βGeo mice. We also specifically tested for interactions between genotype and treatment by linear modeling (Region–Genotype * Treatment) and the only effect found was the Genotype effect. There were no significant differences in volume (absolute or relative) for treatment nor for the interaction of genotype and treatment.

Plotting the AR-42-treated animal’s DNAm values at the 1599 signature sites showed that treatment did not result in large, easily identifiable changes in methylation across the signature, as evidenced by the lack of clustering based on treatment (Fig. 5a). Nonetheless, this did confirm the efficacy of the signature in predicting genotype. To identify differential methylation between vehicle- and AR-42-treated Kmt2d+/βGeo animals, we ran a linear model on the 1599 signature CpGs. Any significant sites would comprise those at which methylation levels were differentially methylated by genotype (i.e., dysregulated in vehicle-treated Kmt2d+/βGeo) and whose methylation status changed by AR-42 treatment (i.e., altered such that the treated KS1 mice had methylation levels more similar to untreated WT than untreated KS1 mice). This analysis of only KS1 mice, vehicle- vs. AR-42-treated identified 3 significant CpGs (Fig. 5b; Additional file 2: Table S5); these sites, at which methylation levels were partially rescued by AR-42-treatment, mapped to three genes Fnbp1, Tpcn1, Hmgcll1. While these genes have not been reported as differentially methylated in individuals with KS1, HMGCLL1, 3-hydroxymethyl-3-methylglutaryl-CoA lyase like 1, in mice and humans enables hydroxymethylglutaryl-CoA lyase activity which, as part of the ketone biosynthesis pathway, generates acetoacetate from hydroxymethylglutaryl-CoA. Acetoacetate is the precursor to 3-hydroxybutryate, an endogenous HDACi shown to have similar ameliorative effects on Kmt2d+/βGeo phenotype as AR-42, when produced via a ketogenic diet [5].

Fig. 5
figure 5

Ar-42 treatment Kmt2d+/βGeo mice rescue a subset of signature CpGs. A Heatmap of signature sites with AR-42 treated samples included, showing that there is no broad methylation effect of treatment (as visualized by dendrogram, with treated samples intermixed with untreated but still clustering by genotype, providing further validation of the signature. B Three CpGs with significant methylation changes in AR-42 treated animals. Asterisks represent significant differential methylation (FDR p-value < 0.05) as tested by limma regression

Of the three “rescued” CpGs, two were originally hypermethylated in Kmt2d+/βGeo and one was hypomethylated; this raised the question of whether AR-42 rescued only gain of methylation by promoting open chromatin with increased histone acetylation, leading to subsequent loss of methylation. We assessed this hypothesis by identifying all signature CpGs at which average AR-42-treated Kmt2d+/βGeo DNAm was closer to average WT methylation than vehicle-treated Kmt2d+/βGeo. Unlike the previous analysis which identified 3 CpGs, we did not apply significance thresholds and assessed only mean group methylation. Of the 1599 signature CpGs, 1100 sites (69%) showed a correction of mean group methylation. This correction was agnostic to the original direction of the methylation change in vehicle-treated Kmt2d+/βGeo, as compared to vehicle-treated WT. In sites originally hypermethylated, 531/769 (69%) were rescued following AR-42 treatment. Similarly, in sites originally hypomethylated, 569/830 (69%) were rescued following AR-42 treatment. Therefore the majority of KS1 signature sites demonstrated a non-significant shift toward WT DNAm levels following 2 weeks of AR-42 treatment.


We identify a blood DNAm signature in a KS1 mouse model, Kmt2d+/βGeo, which contains CpGs sites at which methylation levels correlate with phenotypic severity and are partially rescued by AR-42 treatment. This signature overlaps with the human KS1 signature at 19 genes, with the majority exhibiting shared directional changes between the two species [12]. The differentially methylated loci are also notable in that they mapped to genes that exhibited differential expression in the hippocampus of Kmt2d+/βGeo mice [6]. Together these findings suggest that DNAm signatures carry valuable information related to pathophysiology and treatment but also that they may serve as biomarkers of treatment efficacy. AR-42 has been shown to have a positive effect on learning and memory deficits in Kmt2d+/βGeo mice and also rescues loss of H3K4me3 in the hippocampus [4]. Here, we find a subset of signatures CpGs with significant changes in DNAm levels in AR-42-treated KS1 mice. Furthermore, we find that the majority of CpGs in the signature showed a change in methylation levels indicative of rescue, i.e., the Kmt2d+/βGeo treated group has closer methylation levels to WT than untreated Kmt2d+/βGeo mice.

One interesting feature of the mouse KS1 DNAm signature is the direction of methylation change in Kmt2d+/βGeo. One current hypothesis as to the etiology of KS1 is that the loss KMT2D activity results in an excess of closed chromatin. This is also thought to occur in Kabuki type 2, which is caused by pathogenic variants in KDM6A, a histone demethylase that removes the repressive histone marks H3K27me2/3. Their dysregulation results in highly overlapping clinical presentations, i.e., Kabuki type 1 and 2, and DNAm signatures [12, 13]. While previously assayed changes in histone marks in the Kmt2d+/βGeo mouse support the closed chromatin theory, the DNAm changes do not directly match. One might expect a signature composed of mostly or entirely hypermethylated sites, denoting higher levels of closed chromatin and transcriptional repression; however, both human and mouse KS1-associated loci are composed of both hypo- and hypermethylated sites [12, 14]. This brings into question whether the KS1 DNAm pattern is a direct downstream effect of the loss H3K4 methylation or whether it also encompasses compensatory mechanisms resulting from epistatic mechanisms in the cell. It also highlights our dated view of DNAm as a repressive mark, which is often an oversimplification of a complex biological state, and assumptions that epigenetic cross-talk in disease states is not broken down.

While we observed common DNAm aberrations between the KS1 mouse model and individuals with KS1, an important distinction to take into consideration is the lack of the genetic variation across animals. The only genetic contribution to our derived mouse KS1 signature is the Kmt2d+/βGeo variant. In humans, it is possible that both variant type in the KMT2D and genetic background impact both clinical presentation and DNAm levels at the KS1 signature. For example, missense variants causative of KS1 commonly occur in the SET domain and PHD-type zinc fingers #3 and #4 [40], while a number of reported missense variants in exons 38 and 39 of KMT2D cause a distinct multiple malformations disorder [41]. A small number of phenotype-genotype correlations have been reported in KS1 and further research is required to determine whether these differences translate into measurable differences in DNAm patterns for this disorder [42, 43]. Of note, despite the fact that both our WT and KS1 mice carry no background genetic variation, within each group we observed variability in DNAm patterning in the blood and phenotypic expression, as measured in animal weight and brain volume (Fig. 1; Fig. 4). With respect to disease pathophysiology, this finding supports the hypothesis that some phenotypic differences observed across humans with KS1 may not be related to variant type or genetic background but rather to regulatory changes via epigenetic modifications leading to downstream transcriptional differences.

While there are no significant effects of AR-42 on brain volume in Kmt2d+/βGeo mice following a two-week treatment course, there are strong genotype effects on brain volume, i.e., Kmt2d+/βGeo displays a total brain volume about 10% smaller than WT. A total brain volume change of this magnitude is common in autism-related mouse models, and being that these models are quite heterogeneous, they have a wide range in total brain volume differences [44]. Effect size differences in total brain volume in autism-related mouse models can range from -4 to + 6, and therefore an effect size difference seen here of -3.59 is quite large. These differences are likely connected to developmental delay and/or an arrest of growth. Moreover, microcephaly is considered a supportive clinical feature in the diagnosis of KS1. Relative volume differences give us a further assessment of localized differences comparatively across the brain. Overall, the limbic system seems to be strongly affected in the KS1 mouse model, as the anterior cingulate cortex, pre- or parasubiculum, and hypothalamus displayed significant changes in relative volume; although the hippocampus for the most part is unchanged in relative volume. The hippocampal differences are particularly interesting as previous reports have shown a loss in dentate gyrus volume compared to overall brain weight [4], and while we see an overall decrease of -11% in the dentate gyrus, when compared to overall brain volume that difference becomes insignificant. While that study also did not find a significant difference in overall brain weight, which is inconsistent with our brain volume decrease of 10%, a trend of lower brain weights was observed. The differing reports could be partially explained by the method with which they are measured (i.e., weight vs. volume and immunohistochemistry vs. MRI) and/or the ages at which measurements were taken, but need further study to clarify. Although similar studies in individuals with KS1 is limited, decreased volume of grey matter in KS1 has been reported; volume difference were localized to the bilateral precentral gyrus and middle frontal gyrus [39]. Neuroimaging on individuals with KS1 has also identified structural brain malformations including, abnormal pons and uplifted and hypoplastic vermis [45]. Taken together, these data suggest that while the hippocampus is still a structure of interest for elucidating neurological KS1 features, changes in other structures and both grey and white matter are likely consequential and merit further investigation.

We find brain volume to be significantly associated with 27 signatures sites. Interestingly, the DNAm changes at these CpGs display a linear relationship with brain volume in KS1 mice, but not WT mice, i.e., these associations are specific to the Kmt2d+/βGeo genotype, and support their potential role as biomarkers of KS1 phenotypic severity. In humans there are several or emerging reports of DNAm levels within a signature corresponding to phenotypic severity. For example, Au-Kline syndrome is a neurodevelopmental disorder caused by pathogenic variants in HNRNPK; in 11 of 22 individuals with an Au-Kline diagnosis, tested on the DNAm signature were found to be “intermediate” meaning that their DNAm at signature sites fell between levels that matched individuals carrying HNRNPK loss-of-function variants and levels in healthy controls or individuals with benign variants [46]. Interestingly, these intermediate methylation patterns were primarily identified in individuals who (1) carried an HNRNPK missense variant and (2) presented with a milder clinical presentation, thus indicating a genotype-phenotype-epigenotype correlation [46]. Similarly, in the 22q11.2 deletion syndrome (22q11DS) DNAm signature, individuals carrying a deletion distal to the canonical 22q11.2 deletion, were found to be “control-like” in their DNAm levels and distinct from patterns in individuals with the larger, canonical 22q11.2 deletion [47]. While phenotypes were not available for these individuals, the distal 22q11.2 deletion has been previously associated with a milder phenotype [48]. While both of these examples highlight genotype-phenotype-epigenotype correlations, it is important to note that in the KS1 mice, we observe a phenotype-epigenotype correlation between brain volume and DNAm, independent of genotype as these mice are genetically identical. There are numerous monogenic neurodevelopmental disorders, including 22q11DS, Snijders Blok-Campeau syndrome (CDH3) and KBG syndrome (ANKRD11), with reports of discordant monozygotic twins and/or variable expressivity across individuals in families who inherit the same pathogenic sequence variant [49,50,51]. Moreover, a large-scale study of exome and SNP-array data from ~ 700,000 individuals identified rare loss-of-function and predicted damaging variants in genes associated with monogenic disorders in individuals with subclinical neurodevelopmental phenotypes; these findings highlight further the unmeasured and underreported variable expressivity in this group of disorders [52]. While genetic background and in utero environmental factors contribute to incomplete penetrance, epigenetic mechanisms are likely to have an effect and the possibility of identifying epigenetic patterns corresponding to this clinical variability would fill a large knowledge gap in our understanding of pathophysiology [53].

DNAm signatures have proven valuable in the diagnostic realm, although with any emerging field there are still many questions to address, such as the extent to which DNAm changes in the blood are representative of those in the brain or other tissues. It is also unclear how and when a DNAm signature is established during development. It is also important to consider if the tissue tested demonstrates its own phenotype, for example, individuals with KS1 commonly face immune dysfunction including reduced B cell population [42]. Furthermore, KMT2D has a role in regulating B cell development and its disruption facilitates lymphomagenesis [54]. Given this function in lymphocytes, it is plausible that the DNAm signature resulting for the Kmt2d+/βGeo genotype is affected by these cell types. Kmt2d is expressed in the mouse embryo as early as the two-cell stage (as reported in the MGI database GXD), and so its dysregulation may disrupt DNAm long before cellular differentiation occurs [55, 56]. As such, we hypothesize that this signature likely contains differential methylation patterns (as compared to WT) that are specific to the cells measured, as well patterns that are shared across tissues. The latter may indicate downstream transcriptional dysregulation in other cell types, including neurons and glia. We plan to test this hypothesis with matched blood and brain tissue, which was not possible here as the brain was fixed for imaging.

In sum, this work illustrates how mouse model research into human neurodevelopmental disorders has great utility for understanding disease pathophysiology, and defining optimal treatment approaches as well as developing biomarkers of outcomes for this group of syndromes. While our future studies will undoubtedly benefit from “matched” -omics data, i.e., histone mark and transcriptional measures generated on the same animals in which we assess DNAm and brain volume, we have begun to uncover a clearer picture of KS1 pathophysiology by connecting these molecular marks. As well, given our positive findings for DNAm patterns serving as a biomarker of AR-42 treatment and potentially phenotypic severity, we plan to build on this study and measure DNAm and histone methylation in multiple tissues across the life course of KS1 mice.

Availability of data and materials

Mouse brain volume data and DNA methylation data will be made available on GEO at the time of publication.



DNA methylation


Histone H3 lysine 4


Histone deacetylase inhibitor


Kabuki syndrome type 1


Mendelian disorder of epigenetic machinery


  1. Ng SB, et al. Exome sequencing identifies MLL2 mutations as a cause of Kabuki syndrome. Nat Genet. 2010;42:790–3.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  2. Adam MP, et al. Kabuki syndrome: international consensus diagnostic criteria. J Med Genet. 2019;56:89–95.

    Article  PubMed  Google Scholar 

  3. Adam MP, Hudgins L, Hannibal M. In: Adam MP et al., editors. (Seattle (WA), 1993).

  4. Bjornsson HT, et al. Histone deacetylase inhibition rescues structural and functional brain deficits in a mouse model of Kabuki syndrome. Sci Transl Med. 2014;6:256ra135.

    Article  PubMed  PubMed Central  Google Scholar 

  5. Benjamin JS, et al. A ketogenic diet rescues hippocampal memory defects in a mouse model of Kabuki syndrome. Proc Natl Acad Sci. 2017;114:125–30.

    Article  CAS  PubMed  Google Scholar 

  6. Zhang L, et al. Inhibition of KDM1A activity restores adult neurogenesis and improves hippocampal memory in a mouse model of Kabuki syndrome. Mol Ther Methods Clin Dev. 2021;20:779–91.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  7. Luperchio TR, et al. Leveraging the Mendelian disorders of the epigenetic machinery to systematically map functional epigenetic variation. Elife. 2021;10:e65884.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  8. Chater-Diehl E, et al. Anatomy of DNA methylation signatures: emerging insights and applications. Am J Hum Genet. 2021;108:1359–66.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  9. Choufani S, et al. NSD1 mutations generate a genome-wide DNA methylation signature. Nat Commun. 2015;6:10207.

    Article  CAS  PubMed  Google Scholar 

  10. Rots D, et al. Truncating SRCAP variants outside the Floating-Harbor syndrome locus cause a distinct neurodevelopmental disorder with a specific DNA methylation signature. Am J Hum Genet. 2021;108:1053–68.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  11. Aref-Eshghi E, et al. Genomic DNA methylation signatures enable concurrent diagnosis and clinical genetic variant classification in neurodevelopmental syndromes. Am J Hum Genet. 2018;102:156–74.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  12. Butcher DT, et al. CHARGE and Kabuki syndromes: gene-specific DNA methylation signatures identify epigenetic mechanisms linking these clinically overlapping conditions. Am J Hum Genet. 2017;100:773–88.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  13. Aref-Eshghi E, et al. The defining DNA methylation signature of Kabuki syndrome enables functional assessment of genetic variants of unknown clinical significance. Epigenetics. 2017;12:923–33.

    Article  PubMed  PubMed Central  Google Scholar 

  14. Sobreira N, et al. Patients with a Kabuki syndrome phenotype demonstrate DNA methylation abnormalities. Eur J Hum Genet. 2017;25:1335–44.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  15. Lederer D, et al. Deletion of KDM6A, a histone demethylase interacting with MLL2, in three patients with Kabuki syndrome. Am J Hum Genet. 2012;90:119–24.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  16. Margueron R, Reinberg D. The Polycomb complex PRC2 and its mark in life. Nature. 2011;469:343–9.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  17. Issaeva I, et al. Knockdown of ALR (MLL2) reveals ALR target genes and leads to alterations in cell adhesion and growth. Mol Cell Biol. 2007;27:1889–903.

    Article  CAS  PubMed  Google Scholar 

  18. Montano C, et al. Genome-wide DNA methylation profiling confirms a case of low-level mosaic Kabuki syndrome 1. Am J Med Genet A. 2022;188:2217–25.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  19. Wong CH, Siah KW, Lo AW. Estimation of clinical trial success rates and related parameters. Biostatistics. 2019;20:273–86.

    Article  PubMed  Google Scholar 

  20. Du P, Kibbe WA, Lin SM. lumi: a pipeline for processing Illumina microarray. Bioinformatics. 2008;24:1547–8.

    Article  CAS  PubMed  Google Scholar 

  21. Ritchie ME, et al. limma powers differential expression analyses for RNA-sequencing and microarray studies. Nucleic Acids Res. 2015;43: e47.

    Article  PubMed  PubMed Central  Google Scholar 

  22. Du P, et al. Comparison of Beta-value and M-value methods for quantifying methylation levels by microarray analysis. BMC Bioinformatics. 2010;11:587.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  23. Leek JT, Storey JD. Capturing heterogeneity in gene expression studies by surrogate variable analysis. PLoS Genet. 2007;3:1724–35.

    Article  CAS  PubMed  Google Scholar 

  24. McGregor K, et al. An evaluation of methods correcting for cell-type heterogeneity in DNA methylation studies. Genome Biol. 2016;17:84.

    Article  PubMed  PubMed Central  Google Scholar 

  25. Leek JT, Johnson WE, Parker HS, Jaffe AE, Storey JD. The sva package for removing batch effects and other unwanted variation in high-throughput experiments. Bioinformatics. 2012;28:882–3.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  26. Xu Z, Niu L, Taylor JA. The ENmix DNA methylation analysis pipeline for Illumina BeadChip and comparisons with seven other preprocessing pipelines. Clin Epigenetics. 2021;13:216.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  27. Lerch JP, Sled JG, Henkelman RM. MRI phenotyping of genetically altered mice. Methods Mol Biol. 2011;711:349–61.

    Article  CAS  PubMed  Google Scholar 

  28. Bock NA, Nieman BJ, Bishop JB, Markhenkelman R. In vivo multiple-mouse MRI at 7 Tesla. Magn Reson Med. 2005;54:1311–6.

    Article  PubMed  Google Scholar 

  29. Spencer Noakes TL, Henkelman RM, Nieman BJ. Partitioning k-space for cylindrical three-dimensional rapid acquisition with relaxation enhancement imaging in the mouse brain. NMR Biomed. 2017;30:e3802.

    Article  Google Scholar 

  30. Collins DL, Neelin P, Peters TM, Evans AC. Automatic 3D intersubject registration of MR volumetric data in standardized Talairach space. J Comput Assist Tomogr. 1994;18:192–205.

    Article  CAS  PubMed  Google Scholar 

  31. Avants BB, Epstein CL, Grossman M, Gee JC. Symmetric diffeomorphic image registration with cross-correlation: evaluating automated labeling of elderly and neurodegenerative brain. Med Image Anal. 2008;12:26–41.

    Article  CAS  PubMed  Google Scholar 

  32. Avants BB, et al. A reproducible evaluation of ANTs similarity metric performance in brain image registration. Neuroimage. 2011;54:2033–44.

    Article  PubMed  Google Scholar 

  33. Lerch JP, et al. Automated deformation analysis in the YAC128 Huntington disease mouse model. Neuroimage. 2008;39:32–9.

    Article  PubMed  Google Scholar 

  34. Nieman BJ, Flenniken AM, Adamson SL, Henkelman RM, Sled JG. Anatomical phenotyping in the brain and skull of a mutant mouse by magnetic resonance imaging and computed tomography. Physiol Genom. 2006;24:154–62.

    Article  CAS  Google Scholar 

  35. Dorr AE, Lerch JP, Spring S, Kabani N, Henkelman RM. High resolution three-dimensional brain atlas using an average magnetic resonance image of 40 adult C57Bl/6J mice. Neuroimage. 2008;42:60–9.

    Article  CAS  PubMed  Google Scholar 

  36. Steadman PE, et al. Genetic effects on cerebellar structure across mouse models of autism using a magnetic resonance imaging atlas. Autism Res. 2014;7:124–37.

    Article  PubMed  Google Scholar 

  37. Ullmann JF, Watson C, Janke AL, Kurniawan ND, Reutens DC. A segmentation protocol and MRI atlas of the C57BL/6J mouse neocortex. Neuroimage. 2013;78:196–203.

    Article  PubMed  Google Scholar 

  38. Genovese CR, Lazar NA, Nichols T. Thresholding of statistical maps in functional neuroimaging using the false discovery rate. Neuroimage. 2002;15:870–8.

    Article  PubMed  Google Scholar 

  39. Boisgontier J, et al. Anatomical and functional abnormalities on MRI in kabuki syndrome. Neuroimage Clin. 2019;21: 101610.

    Article  PubMed  Google Scholar 

  40. Faundes V, Malone G, Newman WG, Banka S. A comparative analysis of KMT2D missense variants in Kabuki syndrome, cancers and the general population. J Hum Genet. 2019;64:161–70.

    Article  CAS  PubMed  Google Scholar 

  41. Cuvertino S, et al. A restricted spectrum of missense KMT2D variants cause a multiple malformations disorder distinct from Kabuki syndrome. Genet Med. 2020;22:867–77.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  42. Lindsley AW, et al. Defects of B-cell terminal differentiation in patients with type-1 Kabuki syndrome. J Allergy Clin Immunol. 2016;137:179-187 e110.

    Article  CAS  PubMed  Google Scholar 

  43. Lehman N, et al. Molecular, clinical and neuropsychological study in 31 patients with Kabuki syndrome and KMT2D mutations. Clin Genet. 2017;92:298–305.

    Article  CAS  PubMed  Google Scholar 

  44. Ellegood J, et al. Clustering autism: using neuroanatomical differences in 26 mouse models to gain insight into the heterogeneity. Mol Psychiatry. 2015;20:118–25.

    Article  CAS  PubMed  Google Scholar 

  45. Stadelmaier RT, et al. Neuroimaging in Kabuki syndrome and another KMT2D-related disorder. Am J Med Genet A. 2021;185:3770–83.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  46. Choufani S, et al. An HNRNPK-specific DNA methylation signature makes sense of missense variants and expands the phenotypic spectrum of Au-Kline syndrome. Am J Hum Genet. 2022;109:1867–84.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  47. Rooney K, et al. Identification of a DNA methylation episignature in the 22q11.2 deletion syndrome. Int J Mol Sci. 2021;22:8611.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  48. Rauch A, et al. Systematic assessment of atypical deletions reveals genotype-phenotype correlation in 22q11.2. J Med Genet. 2005;42:871–6.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  49. Singh SM, Murphy B, O’Reilly R. Monozygotic twins with chromosome 22q11 deletion and discordant phenotypes: updates with an epigenetic hypothesis. J Med Genet. 2002;39: e71.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  50. van der Spek J, et al. Inherited variants in CHD3 show variable expressivity in Snijders Blok-Campeau syndrome. Genet Med. 2022;24:1283–96.

    Article  PubMed  Google Scholar 

  51. de Boer E, et al. Missense variants in ANKRD11 cause KBG syndrome by impairment of stability or transcriptional activity of the encoded protein. Genet Med. 2022;24:2051–64.

    Article  PubMed  Google Scholar 

  52. Kingdom R, et al. Rare genetic variants in genes and loci linked to dominant monogenic developmental disorders cause milder related phenotypes in the general population. Am J Hum Genet. 2022;109:1308–16.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  53. Cooper DN, Krawczak M, Polychronakos C, Tyler-Smith C, Kehrer-Sawatzki H. Where genotype is not predictive of phenotype: towards an understanding of the molecular basis of reduced penetrance in human inherited disease. Hum Genet. 2013;132:1077–130.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  54. Zhang J, et al. Disruption of KMT2D perturbs germinal center B cell development and promotes lymphomagenesis. Nat Med. 2015;21:1190–8.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  55. Huang Y, et al. Stella modulates transcriptional and endogenous retrovirus programs during maternal-to-zygotic transition. Elife. 2017;6:e2234.

    Article  Google Scholar 

  56. Ringwald M, et al. Mouse genome informatics (MGI): latest news from MGD and GXD. Mamm Genome. 2022;33:4–18.

    Article  PubMed  Google Scholar 

Download references


The authors would like to acknowledge the members of the Weksberg Lab, especially Chunhua Zhao and Youliang Lou, for their contributions, as well as the Bjornsson Lab and the Mouse Imaging Centre and TCAG staff. We would also like to thank the granting agencies whose funding supported this work, including CIHR and the Ontario Brain Institute-POND study.


This research was funded by a Canadian Institutes of Health Research (CIHR) project grant, “Determining the mechanisms underlying disease pathology in Kabuki syndrome” and the Ontario Brain Institute.

Author information

Authors and Affiliations



S.J.G. performed all DNA methylation analyses, interpreted the data, generated the figures and tables, and wrote the manuscript. T.R.L. helped design the study, performed the mouse work and edited the manuscript. J.E. oversaw the imaging, performed all analysis of brain volume data and interpretation of these data and helped with manuscript writing and editing. E.C.-D. helped design the study, oversee collaborations, assisted with DNA methylation data analysis interpretation, and edited the manuscript. J.L. helped design the study, designed the imaging protocols with J.E. as well as secured funding and helped prepare the manuscript. H.T.B. helped design the study, provided to the mouse strain and oversaw the mouse work, as well as secured funding and helped prepare the manuscript. R.W. is the principal investigator and was involved in all aspects of the study. All authors have read and approved the manuscript.

Corresponding author

Correspondence to Rosanna Weksberg.

Ethics declarations

Ethics approval and consent to participate

All experiments were performed using mouse protocols approved by the Animal Care and Use Committee of Johns Hopkins University School of Medicine. The mouse protocols used for this study are in accordance with the guidelines used by the National Institutes of Health (NIH) for mouse care and handling and the Canadian Council on Animal Care (CCAC). (1) Animal Care and Use Committee of Johns Hopkins University School of Medicine. Animal Use Protocol # MO21M132. (2) Animal Care Committee of The Centre for Phenogenomics. Animal Use Protocol #22-0260H.

Consent for publication

Not Applicable.

Competing interests

H.T.B. is a consultant for Mahzi Therapeutics. R.W. is a consultant for Alamya Health. All other authors declare no competing interests.

Additional information

Publisher's Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary Information

Additional file 1

. Supplementary Figures S1–S5.

Additional file 2

. Supplementary Tables S1–S5.

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit The Creative Commons Public Domain Dedication waiver ( applies to the data made available in this article, unless otherwise stated in a credit line to the data.

Reprints and permissions

About this article

Check for updates. Verify currency and authenticity via CrossMark

Cite this article

Goodman, S.J., Luperchio, T.R., Ellegood, J. et al. Peripheral blood DNA methylation and neuroanatomical responses to HDACi treatment that rescues neurological deficits in a Kabuki syndrome mouse model. Clin Epigenet 15, 172 (2023).

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: