Combinatorial patterns of gene expression changes contribute to variable expressivity of the developmental delay-associated 16p12.1 deletion

Abstract

Background

Recent studies have suggested that individual variants do not sufficiently explain the variable expressivity of phenotypes observed in complex disorders. For example, the 16p12.1 deletion is associated with developmental delay and neuropsychiatric features in affected individuals, but is inherited in > 90% of cases from a mildly-affected parent. While children with the deletion are more likely to carry additional “second-hit” variants than their parents, the mechanisms for how these variants contribute to phenotypic variability are unknown.

Methods

We performed detailed clinical assessments, whole-genome sequencing, and RNA sequencing of lymphoblastoid cell lines for 32 individuals in five large families with multiple members carrying the 16p12.1 deletion. We identified contributions of the 16p12.1 deletion and “second-hit” variants towards a range of expression changes in deletion carriers and their family members, including differential expression, outlier expression, alternative splicing, allele-specific expression, and expression quantitative trait loci analyses.

Results

We found that the deletion dysregulates multiple autism and brain development genes such as FOXP1, ANK3, and MEF2. Carrier children also showed an average of 5323 gene expression changes compared with one or both parents, which matched with 33/39 observed developmental phenotypes. We identified significant enrichments for 13/25 classes of “second-hit” variants in genes with expression changes, where 4/25 variant classes were only enriched when inherited from the noncarrier parent, including loss-of-function SNVs and large duplications. In 11 instances, including for ZEB2 and SYNJ1, gene expression was synergistically altered by both the deletion and inherited “second-hits” in carrier children. Finally, brain-specific interaction network analysis showed strong connectivity between genes carrying “second-hits” and genes with transcriptome alterations in deletion carriers.

Conclusions

Our results suggest a potential mechanism for how “second-hit” variants modulate expressivity of complex disorders such as the 16p12.1 deletion through transcriptomic perturbation of gene networks important for early development. Our work further shows that family-based assessments of transcriptome data are highly relevant towards understanding the genetic mechanisms associated with complex disorders.

Supplementary Information

The online version contains supplementary material available at 10.1186/s13073-021-00982-z.

Background

Complex disorders, such as autism, intellectual disability/developmental delay (ID/DD), epilepsy, and schizophrenia, have been attributed to rare copy-number variants (CNVs), or deletions and duplications encompassing multiple genes, as well as individual rare single-nucleotide variants (SNVs) and the combined effects of common variants [1–6]. Despite advances in high-throughput sequencing methods and quantitative assessments of large cohorts, individual variants implicated for these disorders do not sufficiently explain the variable expressivity and pleiotropy of clinical features often observed in affected individuals [7–9]. An example is the 520-kbp deletion at chromosome 16p12.1 (OMIM: 136570), which was originally described in children with developmental delay [10, 11] but was subsequently found to confer increased risk for schizophrenia [12], epilepsy [13], and cognitive defects in control populations [14]. Unlike syndromic CNVs such as Smith-Magenis syndrome that primarily occur de novo [15], the 16p12.1 deletion is inherited in over 90% of affected children from carrier parents who manifest subclinical or mild cognitive and neuropsychiatric features [10, 16]. In fact, we recently found that children with the deletion were more likely to carry an additional burden of rare CNVs [11] and deleterious variants in genes intolerant to variation [16] elsewhere in the genome compared to their carrier parents. These rare variants in the genetic background, which we define as “second-hit” variants [15], also correlate with the phenotypic presentation of affected children [16], making the deletion an ideal model for assessing the combined effects of multiple variants towards variable clinical outcomes.

While dissecting the pathogenicity of complex disorders has been challenging, cohort and family-based studies that integrate multiple variants with different effect sizes or functional outcomes have provided insights into how the genetic architecture contributes to changes in penetrance, severity, and complexity of phenotypes [17, 18]. In particular, analysis of gene expression patterns in human cells allows for dissecting the direct and indirect effects of genomic variants towards biological functions in complex disorders. For example, Merla and colleagues assessed gene expression in skin fibroblasts and lymphoblastoid cell lines (LCLs) from individuals with the 7q11.23 deletion, associated with Williams syndrome, and found that several genes adjacent to the deletion region were also downregulated compared to controls [19]. Similarly, expression changes due to the autism-associated 16p11.2 deletion correlated with changes in head circumference phenotypes [20] and converged on several neurodevelopmental pathways, including synaptic function and chromatin modification [21]. Other studies have used expression data to identify pathogenic variants potentially missed by genome sequencing studies [22–24]. For example, Frésard and colleagues identified novel causal variants for 6/80 individuals with rare undiagnosed diseases through paired analysis of whole-blood transcriptomes and genomes [22]. Additionally, several recent studies have used family-based approaches to study the effects of rare inherited variants towards gene expression. For example, Pala and colleagues found that rare inherited variants in both coding and non-coding regions increased the likelihood of gene expression changes among 61 families in the bottlenecked Sardinia population, indicating the importance of such variants towards disease risk [25]. While these studies have shown the utility of assessing transcriptomic consequences of individual causal variants, they were focused on either control populations or relatively invariable disorders, and did not examine the simultaneous effects of multiple variants with different effect sizes towards changes in gene expression within major biological pathways.

Here, we integrated whole-genome sequencing and transcriptome data of LCLs from 32 individuals in five large 16p12.1 deletion families who manifested variable phenotypes, in order to investigate how the combined effects of the deletion and “second-hits” perturb transcriptional networks and biological functions. We found that the 16p12.1 deletion disrupts expression of genes involved in neuronal and developmental functions, such as signal transduction and cell proliferation, as well as genes preferentially expressed in the fetal and adult brain. We further identified significant contributions of several classes of rare “second-hit” coding and non-coding variants towards changes in gene expression among carrier children compared with their parents, especially when the variants were inherited from the noncarrier parent. In fact, we found 11 instances of genes in carrier children whose expression was synergistically altered by the combined effects of the 16p12.1 deletion and “second-hit” variants inherited from the noncarrier parent. Although a relatively small sample size precluded global analyses between these expression changes and developmental phenotypes, we found that specific expression changes contributed towards distinct clinical features of affected children through disruption of biological functions related to neurodevelopment. Our results suggest that the 16p12.1 deletion and “second-hit” variants jointly disrupt the developmental transcriptome through shared pathways to contribute towards developmental phenotypes, emphasizing the importance of family-based transcriptome studies for complex disorders.

Methods

Cohort description and recruitment

We obtained clinical data and whole-blood samples from 32 individuals in five families with the 16p12.1 deletion. Among the recruited individuals were 10 children with the deletion (“carrier children”), six sets of carrier and noncarrier parents (including one family with two pairs of parents), three sets of carrier and noncarrier grandparents, and four noncarrier siblings (Additional file 1: Fig. S1; Additional file 2: Table S1). Families with the 16p12.1 deletion, located throughout the USA, were recruited by the Girirajan lab for this study through online patient support groups for the 16p12.1 deletion, in accordance with protocols approved by the Pennsylvania State University Institutional Review Board. Affected children and family members were previously identified as carriers of the deletion through clinical diagnostic tests, which we confirmed using SNP microarray analysis [16]. After providing informed consent, study participants submitted clinical information and primary care providers submitted peripheral blood samples for DNA and B-lymphocyte extraction to the Girirajan lab.

Clinical phenotype analysis

We collected phenotypic information from the five families using two standardized clinical questionnaires: one assessing developmental phenotypes in children, and the other assessing psychiatric features in adults. These data represent comprehensive medical history of affected children and their family members, including neuropsychiatric and developmental features (including cognitive, behavioral, and psychiatric diagnoses), anthropomorphic measures, abnormalities across multiple organ systems (nervous, craniofacial, musculoskeletal, cardiac, hearing/vision, digestive, and urinary systems), and family history of medical or psychiatric disorders. Family members first submitted completed checklists eliciting major phenotypes and medical history, which were then integrated with detailed medical records for each person. A follow-up phone interview was then conducted with family members to fill in any missing information on the clinical questionnaire. Using this method, we assessed clinical data on 31/32 individuals in the cohort. Summarized clinical features for children and adults in this study are listed in Additional file 2: Tables S2-S3. We note that all families had self-reported European or Caucasian ancestry. Based on the curated phenotypic data, we calculated quantitative scores for children using a modified de Vries scoring rubric, as described previously [16], which represents the diversity and severity of phenotypic features in affected children [26]. We similarly summed the number of neuropsychiatric features to generate phenotypic scores in adults. Phenotypic scores for all individuals in the cohort are listed in Additional file 2: Tables S2-S3.

DNA extraction, whole-genome sequencing, and variant identification

We identified 25 classes of rare deleterious variants from whole-genome sequencing (WGS) and SNP microarray for each of the 32 family members in our cohort. The 25 rare variant classes identified in this study are displayed in Additional file 1: Fig. S2 and listed in Additional file 2: Table S4. Genomic DNA was extracted from peripheral blood using QIAamp DNA Blood Maxi extraction kit (Qiagen, Hilden, Germany) and treated with RNAse. DNA levels were then quantified using Quant-iT™ PicoGreen™ dsDNA assay methods (Thermo Fisher Scientific, Waltham, MA, USA), and sample integrity was assessed in agarose gel. After constructing Illumina TruSeq DNA PCR-free libraries (San Diego, CA, USA), whole-genome sequencing was performed on each sample by Macrogen Labs (Rockville, MD, USA) using an Illumina HiSeq X sequencer to obtain an average coverage of 34.5×. Raw sequencing data were processed for quality control using Trimmomatic [27] with leading: 5, trailing: 5, and slidingwindow: 4:20 parameters, aligned to the human hg19 reference genome using BWA v.0.7.13 [28], and sorted and indexed using Samtools v.1.9 [29]. Raw sequencing data and sets of identified variants for all individuals in our cohort have been deposited in the dbGaP repository [30].

The GATK Best Practices pipeline v.3.8 (HaplotypeCaller) and v.4.0.11 (GenotypeGVCFs) [31] was used to identify SNVs and small indels from WGS data. In short, duplicate reads were marked and removed using PicardTools, and after calibration of base-pair quality scores, GATK HaplotypeCaller was used to identify variants in each sample. Variant calls were then pooled for joint genotyping and calibration of variant quality scores. Custom-built pipelines using Annovar v.2016Feb01 [32] applied a total of 430 annotation classes for variant function, population frequency, conservation, genomic region, and predicted pathogenicity. Variants were filtered based on the following quality metrics [33]: QUAL > 50, read depth > 8, allele balance between 0.25 and 0.75 (or > 0.9 for homozygous variants), and quality depth (QUAL/reads with alternate allele) < 1.5. Rare variants were defined as variants with frequency ≤ 0.001 in the gnomAD v.2.1.1 genome database [34], and present in < 10 samples in our in-house WGS cohort of 125 families (335 individuals) with rare CNVs, in order to remove technical artifacts that may be missed by gnomAD. We finally classified rare SNVs and small indels for downstream analysis as follows: rare missense and loss-of-function (LOF, including frameshift and stopgain) variants within protein-coding regions, as well as variants in the 5′ and 3′ untranslated region (UTR) or within 1 kbp of the transcription start (TSS) or end sites (upstream and downstream), were classified based on their RefSeq-defined genomic locations in Annovar (Additional file 1: Fig. S2). Splice-site variants were identified based on MutationTaster annotations [35] for disease-causing (“D”) or disease-causing automatic (“A”) variants. Rare non-coding regulatory variants within 50 kbp of TSS for protein-coding genes were classified according to ChromHMM chromatin state segmentation data for GM12878 lymphoblastoid cells [36], available from the ENCODE Project, into promoters (chromosome states 1–3), enhancers (states 4–7), or silencers (state 12). With the exception of loss-of-function and splice-site variants, all coding and non-coding variants were filtered for CADD Phred-like pathogenicity scores ≥ 10 [37]. Inheritance patterns of these variants were determined using in-house pipelines.

Copy-number variants and structural variants were identified using a combination of WGS data for all samples and SNP microarray data for 25/32 samples, previously described in [16]. Microarray experiments were performed at either the HudsonAlpha Institute for Biotechnology (Huntsville, AL, USA; Illumina Omni 2.5 Exome 8 v1; n = 18), Yale Center for Genome Analysis (New Haven, CT, USA; Illumina OmniExpress 24 v.1.1; n = 5), or the Department of Genome Sciences at the University of Washington (Seattle, WA, USA; Illumina OmniExpress 24 v.1.1; n = 2). Microarray-derived CNV calls for each sample were generated using PennCNV v.1.0.3 [38] and were filtered for ≥ 50 kbp in length and ≥ 5 target probes. CNVs and SVs were also detected from aligned WGS data using a combination of four pipelines: CNVNator v.0.4.1 [39] (bin size of 200), DELLY v.0.8.2 [40], LUMPY-sv v.0.2.13 with Smoove v.0.2.5 [41], and Manta v.1.6.0 [42]. In both WGS and microarray-derived datasets, adjacent CNVs were merged if they overlapped or had a gap < 20% of CNV length and < 50 kbp. We then integrated the CNV and SV calls from each of the datasets as follows: For smaller CNVs and SVs < 50 kbp, any duplication or deletion called by at least two of the four WGS-based callers were considered for downstream analysis, with the minimum intersected regions defining the new breakpoints. For larger CNVs and SVs > 50 kbp, the union of CNVNator and PennCNV calls were considered for downstream analysis. Integrated calls were based on 50% reciprocal overlap among the callers. As our SV call set had a low overlap with SV call sets from control populations, likely due to different SV calling methods used in the control cohorts [43, 44], integrated variants were filtered for presence in < 10 individuals in our in-house WGS cohort, as determined by 50% reciprocal overlap. Finally, RefSeq gene-coding regions spanned by SVs were categorized as follows: encapsulating variants which span the entire gene, interstitial variants that are contained within a gene, and 5′ and 3′ UTR variants that overhang the gene on either end (Additional file 1: Fig. S2). Inheritance patterns of CNV and SV calls were determined if calls in the child and parent had > 50% reciprocal overlap.

Short tandem repeats (STRs) were called from aligned WGS data with GangSTR v.2.4 [45], using the GangSTR hg19 reference file v.13.1. The calls were filtered and analyzed using three tools from the STR analysis toolkit TRTools [46]. First, dumpSTR was used to filter for quality of calls using the following parameters: read depth > 20, read depth < 1000, QUAL > 0.9, spanbound only (calls that are spanned by reads), and filter bad confidence intervals (filtered calls whose maximum likelihood estimates were not within the confidence interval). The reads were then merged with mergeSTR, and basic statistics were calculated using statSTR. In addition to the dumpSTR filters, we applied the following filters to our call set: > 95% of samples called for the STR location, variance at location > 0, and overlap of the STR location with a RefSeq-defined protein-coding gene. STR expansions were defined as any call for which the deviation of the repeat length was greater than the mean length plus three standard deviations among all individuals in our cohort. Finally, STR variants were categorized according to their genomic location, including exonic, intronic, 5′ or 3′ UTR, upstream, and downstream (Additional file 1: Fig. S2). Inheritance patterns of STRs were determined by matching the number of repeats in the child to their parents.

Generation of lymphoblastoid cell lines and RNA sequencing

Peripheral blood samples for all 32 individuals in our cohort were submitted to the Coriell Institute for Medical Research (Camden, NJ, USA) for generation of lymphoblastoid cell lines through Epstein-Barr virus transformation of B lymphocytes (Additional file 2: Table S5). After receiving the LCL samples, cells were grown at 5% CO₂ and a concentration of 1× 106 cells/mL under L-glutamine-supplemented RPMI 1640 medium (11875-119, Thermo Fisher Scientific) containing 15% fetal bovine serum (35-010-CV, Corning Life Sciences, Tewksbury, MA, USA) and Cytiva HyClone™ Penicillin Streptomycin solution (SV30010, Thermo Fisher Scientific). Total RNA was isolated from three biological replicates of P6-P7 cells per sample using TRIzol Reagent (Thermo Fisher Scientific) and PureLink RNA Mini Kit (12183018A, Thermo Fisher Scientific), and subsequently treated with DNA-free DNA Removal Kit (AM1906, Thermo Fisher Scientific). RNA integrity number scores (RIN) were assessed using Agilent Bioanalyzer 2100 (Additional file 1: Fig. S3A), and replicates with RIN scores > 8.5 were sequenced. Paired-end 50 bp libraries for each replicate were generated using Illumina TruSeq Stranded mRNA kit and were sequenced using Illumina NovaSeq at the Penn State College of Medicine Genome Sciences Facility (Hershey, PA, USA). Two sequencing runs of 48 replicates were performed, with the biological replicates of each sample split among the two runs to mitigate batch effects, to generate a total of 43.5 million reads/replicate. Raw sequencing data and quantified expression values for all LCL samples have been deposited in the dbGaP repository [30].

Quantification of gene expression and coverage of disease genes

Sequenced RNA reads were filtered using Trimmomatic v.0.36 [27] to remove reads <30 bp long. Following the GTEx Consortium RNA-seq pipeline [47], the filtered reads were aligned to the human genome (GENCODE v.19) using STAR v.2.4.2a [48], and sorted and indexed using Samtools v.1.9 [29]. Duplicates reads were marked with PicardTools v.2.9.0. We assessed the quality of the aligned reads with transcript integrity scores [49], which moderately correlated (r = 0.38, p = 1.0 × 10⁻⁴, Pearson correlation) with the RIN scores for each sample (Additional file 1: Fig. S3A). Isoform counts for GENCODE 19 genes were quantified using RSEM v.1.2.22 [50]. A collapsed gene coordinate GTF file was generated using the GENCODE 19 gene coordinates and the GTEX collapse_annotation script. Gene-level counts and transcripts per million read (TPM) values were quantified using RNASeQC v.1.1.8 [51], using strict mode and the collapsed gene coordinates.

After filtering for transcripts where all three replicates of at least one sample showed > 0.2 TPM, we obtained a total of 24,340 expressed transcripts across our cohort, representing 43.3% of all GENCODE transcripts. We further compared our set of expressed LCL genes to disease gene databases [52–56] and genes expressed in the adult brain from GTEx consortium RNA-seq data [47]. We defined expressed genes in GTEx tissues if they showed > 0.5 TPM in 80% of samples for a particular tissue. The expressed LCL genes covered > 70% of each of these gene sets, including 83% of genes expressed in GTEx brain tissues (Additional file 1: Fig. S4A-B). These data are in concordance with gene expression data from GTEx, where gene expression values in LCLs and brain tissues showed an average Spearman correlation of 0.84 (Additional file 1: Fig. S4C). These findings indicate that our LCL data would be able to identify changes in expression patterns for most genes related to neurodevelopmental disease.

Differential expression and outlier expression analysis

We performed differential expression analysis between all 16p12.1 deletion carriers and noncarriers, as well as between parents and offspring across the five families, using edgeR [57] v.3.30.0 on gene-level counts to create generalized linear models and perform quasi-likelihood F-tests with Benjamini-Hochberg correction. For testing differences between all deletion carriers (n = 19) and noncarriers (n = 13), we included family as a covariate in the linear model, used default filtering for low-expressed genes, and removed genes with sex-specific differences in GTEx LCL samples as well as genes on the X and Y chromosomes (due to unequal sex ratios in deletion carriers and noncarriers). To control for expression outliers, we iteratively identified sets of differentially expressed genes, defined using an FDR < 0.05 threshold (Benjamini-Hochberg correction), between deletion carriers and noncarriers after removing one sample at a time. We then took the intersection of the resulting 32 sets of differentially expressed genes, and obtained a total of 1569 transcripts differentially expressed in the deletion carriers (Additional file 3: Data S1). We also performed differential expression analysis using PQLseq v.1.2 to account for gene expression similarity due to relatedness [58]. We first generated input files from unfiltered WGS SNV data using PLINK v.1.9 [59], and used GEMMA v.0.98.3, which calculates kinship between two individuals based on genotype similarity [60], to generate a kinship matrix for our cohort. This matrix was used as input for PQLseq along with gene-level counts from RNA-seq data, after removing the same sex-specific genes as for the edgeR analysis.

We next performed family-based analysis on 13 separate trios identified across the five families (nine carrier children compared to parents and four carrier parents compared to grandparents), which are listed in Additional file 2: Table S1. For example, we separately analyzed two trios in family GL_001 (Additional file 1: Fig. S1). For comparison, we analyzed an additional four trios with noncarrier children compared to carrier and noncarrier parents (Additional file 1: Fig. S5C). For each trio, we first used an edgeR workflow without covariates to identify differentially expressed genes between the offspring and carrier parent (|logFC| > 0.5, FDR < 0.05, Benjamini-Hochberg correction), and separately assessed expression changes between the offspring and noncarrier parent. Genes with low expression (expressed in < 25% of all replicates) and sex-specific genes were removed from edgeR analysis. We then overlapped the two sets of differentially expressed genes to classify expression changes by family-specific patterns as follows: “unique” if the gene was differentially expressed in the offspring compared with both parents; “shared with the carrier parent” if the gene was only differentially expressed compared with the noncarrier parent; and “shared with the noncarrier parent” if the gene was only differentially expressed compared with the carrier parent (Additional file 1: Fig. S5A).

To identify genes with outlier expression in our cohort, we calculated z-scores of gene expression values for each individual for 14,212 protein-coding genes expressed in the LCL samples. We normalized the expression values in each person by calculating the median TPM expression across the three replicates for each gene, transformed the values using log₂(x + 1), and calculated z-scores for each log-transformed TPM compared with all samples in our cohort. As principal component analysis showed clustering of samples by family (Additional file 1: Fig. S6A), we used PEER v.1.0 [61] to correct the z-scores using one PEER principal component (Additional file 1: Fig. S6B). After correction, we further assessed for clustering of samples and replicates, and found strong Spearman correlations among replicates derived from the same sample (Additional file 1: Fig. S3B). We defined outlier genes as any gene with |z-score| > 2 (Additional file 1: Fig. S6C), in line with recent studies utilizing outlier expression values [22].

Enrichment analysis for biological function, brain expression, and disease relevance

Enrichment analysis for sets of differentially expressed genes was performed using goseq v.3.12 [62], which tests for overrepresentation of gene categories in RNA-seq data. Goseq controls for selection bias in RNA-seq datasets by modeling the distribution of transcript lengths of differentially expressed genes. We assessed for enriched biological processes using the Gene Ontology database [63], as well as genes expressed in specific adult brain tissues from GTEx [47] and developing brain tissues from the BrainSpan Atlas [64]. We defined preferentially expressed genes in GTEx and BrainSpan tissues as expression > 2 standard deviations higher than the median expression across all tissues for that gene. We further assessed for enrichment of differentially expressed gene sets for candidate neurodevelopmental disease genes (DBD Gene Database) [52], as well as specific gene sets for autism (SFARI Gene database) [53], intellectual disability (DDD and DDG2P databases) [55, 56], and schizophrenia [54]. Finally, we annotated sets of genes with altered expression for two common measures of intolerance to variation, RVIS [65] and pLI [66], and used genes considered to be intolerant to variation (RVIS < 20th percentile or pLI score > 0.9) for downstream analysis. All gene sets used for enrichment analyses were filtered for genes with transcripts that are expressed in our LCL samples (> 0.2 TPM in all three replicates of at least one sample).

PAGE and WGCNA analysis in deletion carriers and noncarriers

We performed parametric analysis of gene set enrichment (PAGE) on genes that were differentially expressed between carriers and noncarriers of the 16p12.1 deletion [67]. PAGE is a gene set analysis method that considers the direction of the expression log fold change to discover sets of genes that are enriched among up- or downregulated genes. For this analysis, we included the log fold change of 26,861 transcripts that were not filtered out by edgeR’s default filtering of low-expressed transcripts. We searched for significant up- or downregulation of genes within terms from the Gene Ontology database [63], using two-tailed z-tests with Benjamini-Hochberg correction.

We further performed weighted gene correlation network analysis (WGCNA) to identify modules of genes that were co-expressed among samples in our cohort [68]. We used the R package tximport [69] to import RSEM-derived gene expression counts, filtered genes for > 10 counts/replicate in at least one sample, and used DESeq2 [70] to generate variance-stabilized expression counts for each gene. To detect co-expression patterns specific to deletion carriers, we used ComBat [71] within sva v.3.12 to perform batch correction with family as a covariate. We detected 35 co-expression modules in our samples using WGCNA v.1.69 [68], with the following parameters: power threshold = 8, signed hybrid network, unsigned topological overlap matrix, bi-weight mid-correlation, module size = 30–30,000, and merge cut height = 0.25. Two modules showed strong sex-specific gene expression and were excluded from further analysis. The average gene expression values in each module were compared between carriers and noncarriers using two-tailed t tests, and genes in each of these modules were tested for enrichment of Gene Ontology terms using goseq.

Integration of gene expression and genomic variant data

We calculated the effect size of different classes of rare “second-hit” variants towards gene expression changes, stratified by sample type and family-specific patterns. We compared 25 classes of rare variants identified from WGS data (Additional file 1: Fig. S2; Additional file 2: Table S4) towards differentially expressed genes in family trios as well as outlier expression genes in all individuals. For all comparisons, we calculated odds ratios and 95% confidence intervals for each variant class towards changes in expression using Fisher’s exact and Wald tests, respectively; uncorrected p values and Benjamini-Hochberg-corrected FDR values were reported for each comparison (Additional file 4: Data S2). We note that we considered each variant class independently, so that dysregulated genes with multiple types of disrupting variants were counted within multiple variant classes. For the differential expression analysis, we first assessed variants in the 13 trios with carrier offspring for genes with differential expression (Additional file 2: Table S1), and then determined the effects of variants in carrier children (n = 9 trios) inherited from carrier or noncarrier parents towards expression changes shared with the same parent. For the outlier expression analysis, we first assessed variants for outlier expression genes in all individuals. We then stratified these data by sample type (carrier child, carrier parent, and noncarrier parent), and compared variants in carrier children that were inherited from their carrier or noncarrier parent. To identify synergistic effects between the 16p12.1 deletion and “second-hit” variants, we identified a subset of genes with outlier expression in deletion carriers that were also differentially expressed in the global comparison of carriers and noncarriers, and then identified those genes which also had “second-hit” variants inherited from the noncarrier parent.

Alternative splicing analysis

To assess alternative splicing events from RNA sequencing data, we used DESeq2 [70] to detect differential expression of isoforms. After importing isoform-level expression counts from RSEM using tximport [69], we filtered for genes with > 2 counts across all samples and performed pairwise comparisons between carrier offspring and their parents in the 13 trios listed in Additional file 2: Table S1, plus the four trios with noncarrier children for comparisons. We then repeated the DESeq2 analysis for gene expression counts, and only included differentially expressed isoforms within genes that did not show overall differential expression, to specifically account for isoform changes due to alternative splicing. Similar to the family-based differential expression analysis, we assigned family-specific patterns to each alternative splicing event observed in offspring based on the pairwise comparisons to each parent. We further compared alternate isoforms identified by DESeq2 to those in GTEx LCL data [47] to identify unique isoforms in our cohort. Finally, we integrated these data with 12 classes of putative splice-site disrupting variants identified from WGS data and calculated odds ratios as described above.

Allele-specific expression analysis

We used the phASER v.1.1.1 [72] pipeline to identify allele-specific expression events in our cohort. We first used whatshap v.0.18 [73] to perform read-backed and pedigree-informed phasing of our WGS samples, and then merged the three replicate BAM files of aligned RNA-seq reads for each sample together using Samtools. We then used phASER, which uses phased WGS data to infer phasing of RNA-seq samples, to phase the RNA-seq alignments and to count the number of reads per haplotype block. We ran phASER with the parameters --mapq 255 and --baseq 10, and used the recommended blacklist to remove HLA genes. Finally, we quantified log-fold changes for allelic counts in each protein-coding gene with > 10 read counts using phASER Gene AE and identified ASE for genes with FDR > 0.05 using binomial tests with Benjamini-Hochberg correction. For each identified ASE event, we examined the overexpressed haplotype for presence of a deleterious rare coding variant identified from WGS, which would potentially indicate pathogenic effects of the ASE event. Finally, we determined family-specific patterns of ASE genes based on the presence of ASE in parents of offspring.

eQTL discovery and analysis

We used QTLTools v.1.2 [74] to identify eQTLs in our cohort. Because we had three replicates per participant, we first calculated the median TPM values for all transcripts in an individual. Genes were filtered for > 0.1 median TPM in more than 50% of samples. Principal components for gene expression (from RNA-seq data) and genotype (from whatshap-phased WGS data) were then computed using QTLtools. The top three genotype and the top two gene expression principal components were used as covariates for the linear model, in addition to three explicit covariates (family, sex, and carrier status). QTLtools cis-permutation tests (n = 1000 replicates) were then used to discover eGenes, or genes whose expression are significantly correlated with eQTLs, and associated variants in our samples. We performed multiple-testing correction with the QTLtools script runFDR_cis.R. Finally, we annotated significant eQTL variants (FDR < 0.05) associated with protein-coding genes for presence in GTEx LCL data, genomic location, population frequency, and biological functions using the WGS Annovar-based pipeline [32].

Brain-specific network analysis

We assessed the connectivity patterns of genes with “second-hit” variants and changes in expression in the context of a brain-specific interaction network. The network contains brain-specific pairwise interactions for 14,763 genes expressed in the brain, of which 11,978 (81.1%) are also expressed in the LCL samples. This network was previously built using a Bayesian classifier trained on hundreds of gene co-expression, protein-protein interaction, and regulatory-sequence datasets, in order to predict the likelihood of interactions between any two pairs of brain-expressed genes [75, 76]. To create a network containing only the highest probability predicted gene interactions, we extracted all pairs of genes with weighted probabilities > 2.0, representing the top ~ 0.5% of pairwise interactions (217,975,718 pairs of genes). We then calculated the weighted shortest path lengths for all pairs of genes in the network, using the inverse of the probabilities as weights for each edge. Finally, we created sub-networks that contained genes with “second-hit” protein-coding variants (loss-of-function or LOF, missense, splice-site, exonic STR, or encapsulated deletion or duplication) or expression changes (differential expression, outlier expression, alternative splicing, ASE, or eQTL minor allele) for each carrier offspring from the 13 trios (Additional file 2: Table S1). For each trio, we calculated the average shortest paths between all pairs of genes with expression changes and genes with “second-hit” coding variants, and then compared these distances to average shortest paths calculated from 100 permuted network replicates, where genes were randomly reassigned to different nodes in networks with otherwise identical topology. Network analysis was performed using the NetworkX package in Python [77].

Statistical analysis

All genomic and statistical analyses were conducted using either Python v.3.7.3, with packages numpy v.1.16.2 [78], scipy v.1.1.0 [79], and pandas v.1.0.0 [80], or using R v.3.5.1 (R Foundation for Statistical Computing, Vienna, Austria). Details of all statistical tests, including summary statistics, test statistics, odds ratios, confidence intervals, p values, and Benjamini-Hochberg-corrected FDR values, are provided in Additional file 4: Data S2.

Results

The 16p12.1 deletion leads to pervasive disruption of genes involved in neurodevelopment

We performed RNA sequencing on LCL samples from 19 deletion carriers and 13 noncarriers from five large families with multiple affected members (Fig. 1; Additional file 1: Fig. S1; Additional file 2: Table S1) [30], and identified 1569 transcripts that were differentially expressed (FDR < 0.05) in deletion carriers compared with noncarriers (Fig. 2A, B; Additional file 3: Data S1). Application of additional corrections for relatedness among the samples [58] (see “Methods”) yielded 1044 differentially expressed transcripts, of which 840 (80.5%) were also identified in the main analysis (Additional file 1: Fig. S7A; Additional file 3: Data S1). We first confirmed that each of the seven protein-coding genes in the deletion region were downregulated in deletion carriers (Fig. 2C). Interestingly, 13 protein-coding genes adjacent to the 16p12.1 region (between chromosomal bands 16p11.2 and 16p12.3) also showed differential gene expression in carriers, 10 of which were under-expressed in the deletion carriers. For example, two genes within the autism-associated 16p11.2 region, SEZ6L2 and DOC2A, as well as the febrile seizure-associated gene STX1B [83], were downregulated in carriers of the 16p12.1 deletion. As none of the carriers harbored an atypical deletion, it is possible that these adjacent genes could be affected by disruption of regulatory elements located within the deletion region. In fact, three downregulated genes adjacent to the deletion, DNAH3, OTOA, and NPIPB4, exhibited chromatin interactions with enhancer elements within the deletion region, detected using published Hi-C data of LCL samples [81] (Fig. 2C).

Fig. 1.

Overview of experimental design. We performed whole-genome sequencing, RNA sequencing, and clinical phenotyping on five large families (32 total individuals) with the 16p12.1 deletion, indicated with red asterisks in the pedigrees. Children (green) and adults (blue) in the pedigrees are shaded by phenotypic severity score, with white indicating no clinical features, lighter shades indicating mild features (child de Vries score of 1-4; adult score of 1–2 features), medium shades indicating moderate features (child de Vries score of 5–8; adult score of 3–4 features), darker shades indicating severe features (child de Vries score of 9–13; adult score of 5–6 features), and grey indicating no phenotypic data available. Phenotypic severity scores are described in the Methods and are listed for each person in Additional file 2: Tables S2-S3. We then performed multiple analyses to assess the role of the deletion and rare “second-hit” variants towards the observed transcriptomic changes and developmental phenotypes, including differential expression between carriers and noncarriers of the deletion, differential expression between parents and carrier offspring in 13 trios from the five families, outlier gene expression among all individuals, identification of additional transcriptomic alterations such as alternative splicing and allele-specific expression, and gene interaction patterns in the context of a brain-specific network

Fig. 2.

Differential expression of genes between carriers and noncarriers of the 16p12.1 deletion. A Volcano plot showing downstream (non-16p12.1 deletion) genes differentially expressed (FDR < 0.05) between carriers (n = 19) and noncarriers (n = 13) of the deletion. Red circles indicate genes preferentially expressed in GTEx cerebral cortex tissues. B Scatter plot showing all genes differentially expressed between carriers and noncarriers of the deletion by chromosome, excluding genes on sex chromosomes. Genes are colored by FDR of differential expression. Labeled genes indicate candidate autism genes with differential expression. C Expression changes and chromatin connectivity of genes within the 16p12.1 region. The top plot shows pairwise chromatin interactions within the 3.5 Mbp 16p12.1 region, with red lines representing stronger Hi-C intensity, while the bottom plot shows log₂-fold change of expression in deletion carriers of genes within and adjacent to the 16p12.1 deletion. The Hi-C data is from previously reported Hi-C experiments of LCL samples [81], and the heatmap was generated using the 3D Genome Browser [82]. D Line plot shows enrichment (log₁₀ FDR) of differentially expressed genes in deletion carriers for genes preferentially expressed in six select BrainSpan tissues across 11 developmental timepoints

We found that differentially expressed genes in deletion carriers were enriched (FDR < 0.05) for multiple biological functions, including biological adhesion and cell proliferation regulation for relatedness-corrected genes, and signal transduction and locomotion for genes without relatedness correction (Additional file 3: Data S1). Additionally, we observed an enrichment (FDR = 0.015) for candidate autism genes [53], including FOXP1, CUL7, ANK3, and EP300, among the differentially expressed genes (Fig. 2B; Additional file 3: Data S1). Parametric Analysis of Gene Set Expression (PAGE) showed that genes related to neuronal and muscular growth functions were significantly upregulated in deletion carriers (FDR < 0.05), while genes involved in behavioral responses and learning were downregulated (Additional file 1: Fig. S7B; Additional file 2: Table S6). Weighted-gene correlation network analysis similarly identified several modules of genes with significant expression changes in deletion carriers (p < 0.05, two-tailed t-test), including downregulated genes enriched for cell signaling and adhesion, and upregulated genes enriched for neurogenesis, nervous system development, and MAPK and Notch signaling (Additional file 1: Fig. S8; Additional file 5: Data S3). Differentially expressed genes in deletion carriers were further enriched (FDR < 0.05) for genes preferentially expressed in the hippocampus and basal ganglia of the adult brain [47] (Additional file 1: Fig. S7C; Additional file 3: Data S1), as well as in the striatum, thalamus, and frontal cortex during late fetal and adolescent/young adulthood timepoints [64], which are critical transition periods for expression of neurodevelopmental genes [84–86] (Fig. 2D; Additional file 3: Data S1). Overall, our data suggest that the 16p12.1 deletion leads to pervasive transcriptomic changes across multiple biological and neuronal processes in the developing brain. We note that because these results are based on expression data from LCL samples, they should be followed up in neuronal models to delineate any tissue-specific differences in gene expression.

Family-specific patterns of gene expression changes influence developmental phenotypes

We next investigated how gene expression patterns segregated within 13 complete trios with carrier offspring extracted from the five families, including carrier children compared to their parents as well as carrier parents compared with grandparents (Additional file 2: Table S1). For each trio, we identified differentially expressed genes for offspring-carrier parent and offspring-noncarrier parent pairs (see “Methods”), and found an average of 5323 total gene expression changes in offspring compared to their parents (Additional file 2: Table S7; Additional file 6: Data S4). We then overlapped the two sets of differentially expressed genes to categorize expression changes based on their family-specific pattern (Additional file 1: Fig. S5A). We found no significant differences (p = 0.735, two-tailed paired Mann-Whitney test) in the proportion of differentially expressed genes in offspring that were shared with either the carrier (avg. 2223 genes/offspring) or noncarrier parent (avg. 1908 genes/offspring; Fig. 3A). This may suggest that “second-hit” variants from the noncarrier parent could contribute equally to gene expression changes, and therefore to disease pathogenicity, as the combined effects of the deletion and any “second-hit” variants from the carrier parent, an observation that corresponds with our recent findings of increased burden of “second-hits” transmitted to the child from noncarrier parents [16] (Additional file 1: Fig. S5B). However, we also note that this study may be under-powered to detect smaller differences in the proportion of gene expression changes shared between offspring and their carrier and noncarrier parents. Interestingly, we also observed an average of 1192 genes/offspring that were differentially expressed compared with both parents (Fig. 3A), such as SHANK2, FOXP1, and CACNA1D. These expression changes potentially represent effects of de novo variants or combinatorial effects of variants inherited from both parents, which could explain the increased phenotypic severity observed in the carrier children. However, the trends in expression patterns widely varied across families, which in some cases could be explained by family history of neuropsychiatric disease (Additional file 1: Fig. S5C). For example, we found that children within family GL_004, whose parents were unaffected or presented with mild depression, had the lowest number of gene expression changes among any carrier children in the cohort. Meanwhile, children in families GL_001 and GL_052, whose carrier parents manifested multiple overt cognitive and neuropsychiatric features, had higher proportions of expression changes shared with their carrier parents compared to their noncarrier parents (Additional file 1: Fig. S5C).

Fig. 3.

Differential expression of genes between offspring and carrier and noncarrier parents. A Boxplot shows the proportion of differentially expressed genes in carrier offspring of 13 trios (Additional file 2: Table S1) that were either unique to the offspring or shared with their carrier or noncarrier parents (*p < 0.05, two-tailed paired Mann-Whitney test). Boxplot indicates median (center line), 25th and 75th percentiles (bounds of box), and minimum and maximum (whiskers). B Table shows observed clinical features in eight carrier children with overt developmental phenotypes, as well as enrichments (FDR < 0.05) of differentially expressed genes in each carrier child for biological functions related to each clinical feature. Cells are colored according to the family-specific patterns (uniquely observed or shared with a parent) of differentially expressed genes for each enriched biological process

We next assessed the dysregulated biological functions in each trio (Additional file 1: Fig. S9; Additional file 6: Data S4) and found that unique or shared differentially expressed genes in carrier children were enriched for biological processes (FDR < 0.05) that could be related to 33 out of 41 (80.5%) developmental phenotypes observed in the affected children (Fig. 3B). For example, shared gene expression changes for carrier child P1C_01 in family GL_001 were enriched for nervous system development, neurotransmitter metabolism, neuron projection, and synaptic transmission functions, while their unique expression changes were enriched for genes involved in skeletal and muscular development. The shared changes in neuronal genes could contribute to the ID/DD and speech delay phenotypes observed in the child, as both parents also had several psychiatric features, while the unique changes in developmental genes could be related to hypotonia, growth delay, and craniofacial features uniquely observed in the child. Overall, these results suggest that expression changes of neurodevelopmental-related genes could account for phenotypic differences among carriers of the 16p12.1 deletion.

“Second-hit” variants and the 16p12.1 deletion show synergistic effects towards gene expression

We next investigated whether changes in gene expression could be attributed to “second-hits”, or rare genetic modifiers elsewhere in the genome. Rare variants disrupting protein-coding regions and nearby regulatory elements have been previously linked to gene expression changes in both control populations [25, 87–89] and disease cohorts, where causal genes may be missed by DNA sequencing methods [20, 22–24]. We hypothesized that “second-hits” by themselves or in combination with the deletion could contribute to the observed gene expression changes in affected children. We therefore identified 25 classes of rare gene-disruptive “second-hit” variants from WGS data for each individual (Additional file 1: Fig. S2; Additional file 6: Data S4; Additional file 7: Data S5) [30], including SNVs and indels in coding and non-coding regulatory regions (UTRs, introns, and putative promoter, enhancer, and silencer elements within 50 kbp of a gene) with Phred-like CADD scores > 10 [37], and CNVs and short tandem repeats (STRs) that spanned gene-coding regions. We then calculated the likelihood that these “second-hit” variants are associated with changes in expression of a proximal gene, as determined by either differential expression analysis between carrier offspring and their parents in the 13 trios, or outlier expression analysis among all individuals in the cohort [20, 87] (see “Methods”). While family-based differential expression analysis detects all expression changes between affected children and their parents [90], including those due to the downstream effects of the deletion, outlier analysis more robustly identifies specific effects of “second-hits” towards larger changes in expression, including synergistic effects in combination with the deletion. Overall, we observed an average of 285 outlier genes (|z-score| > 2) per individual, including candidate neurodevelopmental genes [52] such as CTNNB1, FOXG1, DISC1, and ZNF804A (Additional file 1: Fig. S6; Additional file 2: Table S7; Additional file 8: Data S6). We found that 10.8% of outlier genes (avg. 31/286 per person) and 11.2% of differentially expressed genes (avg. 310/2774 per carrier offspring) were potentially disrupted by a rare coding or non-coding variant (Additional file 7: Data S5). Altered expression of genes without such variants could be due to several factors, such as common variants, DNA methylation events, downstream effects of other dysregulated genes, or environmental factors.

In agreement with previous studies [25, 87], we found that genes with outlier expression were significantly enriched after Benjamini-Hochberg correction (FDR < 0.05, Fisher’s exact test) for 5/25 classes of rare variants that directly affected gene-coding regions, including loss-of-function (LOF), missense, and splice-site SNVs, and 5′ UTR overhanging and gene-encapsulating duplications (Fig. 4A). Similarly, we found that 10/25 variant classes were significantly associated with differentially expressed genes in carrier offspring for the 13 trios (FDR < 0.05, Fisher’s exact test), including coding missense SNVs, duplications overhanging the 5′ UTR, and encapsulated deletions (Additional file 1: Fig. S10A). We further found that outlier genes had higher burdens of rare variants in aggregate (p = 1.01 × 10⁻³, one-tailed t-test) and for 7/25 individual classes compared with non-outlier genes (p < 0.05, one-tailed t-test), in particular loss-of-function variants (FDR = 1.73 × 10⁻³) and encapsulated duplications (FDR = 5.43 × 10⁻³), which passed multiple-testing correction (Additional file 1: Fig. S11A-B). Interestingly, we also found that outlier genes that were intolerant to variation (pLI score > 0.9 or RVIS percentile < 20; p < 3.26 × 10⁻⁴, two-tailed t-test) or preferentially expressed in the brain (p = 0.011) had a higher burden of nearby rare variants than other outlier genes (Additional file 1: Fig. S11C). We next assessed the effect size of “second-hits” towards outlier gene expression among carriers and noncarriers of the deletion, and found enrichments of LOF variants (p = 4.96 × 10⁻⁶; FDR = 6.20 × 10⁻⁵), 5′ UTR overhanging duplications (p = 0.017; FDR = 0.108), and 5′ UTR-disrupting SNVs (p = 7.37 × 10^-3; FDR = 0.058) towards outlier expression in carrier children but not in carrier parents (Fig. 4B). We observed similar findings among differentially expressed genes, where missense SNVs (FDR = 4.23 × 10⁻⁵), upstream SNVs (FDR = 7.00 × 10⁻⁴), encapsulated (FDR = 0.039) and interstitial (FDR = 0.031) deletions, and 5′ UTR overhanging duplications (FDR = 0.045) were only likely to alter gene expression in carrier children (Additional file 1: Fig. S10B). Notably, LOF variants (p = 1.67 × 10⁻⁵, FDR = 2.09 × 10⁻⁴) and 5′ UTR overhanging duplications (p = 0.018; FDR = 0.090) were also enriched for outlier expression in noncarrier parents, suggesting that these classes of “second-hit” variants were more likely to be deleterious in carrier children when inherited from noncarrier parents (Fig. 4B). In fact, we observed several classes of “second-hit” variants in carrier children, including 5′ UTR overhanging duplications (p = 1.54 × 10⁻³, FDR = 0.025), gene-encapsulating (p = 0.025; FDR = 0.125) and 3′ UTR overhanging deletions (p = 0.025; FDR = 0.125), and missense (p = 0.023; FDR = 0.125) and upstream SNVs (p = 0.032; FDR = 0.133), that were enriched for outlier expression when inherited from the noncarrier parent but not from the carrier parent (Fig. 4C). Similarly, we found that LOF variants (FDR = 5.05 × 10⁻⁵) and SNVs in upstream (FDR = 6.25 × 10⁻³) and silencer regions (FDR = 7.70 × 10⁻⁴) correlated with differential gene expression in carrier children only when inherited from the noncarrier parent (Additional file 1: Fig. S10C). For example, a carrier child in family GL_007, who exhibited hypotonia and muscle weakness, inherited a deleterious variant from their noncarrier parent in the 5′ UTR of EIF2AK1, associated with motor dysfunction [91], that potentially led to downregulation of that gene (Fig. 4D). Overall, our findings showed that distinct classes of “second-hit” variants differentially contribute towards changes in gene expression when inherited in a complex manner from either the carrier or noncarrier parent.

Fig. 4.

Enrichment of “second-hit” variants near genes with outlier expression. A Forest plot shows enrichment (Fisher’s exact test, ** = FDR < 0.05, * = uncorrected p < 0.05) of genes with outlier expression in all individuals in the cohort (n = 32) for rare proximal coding and non-coding variants, including single-nucleotide variants (SNVs) and insertions/deletions (indels) with CADD scores > 10 [37], structural variants (SVs), and short tandem repeats (STRs). B Forest plot shows classes of “second-hit” variants with significant enrichment (Fisher’s exact test, ** = FDR < 0.05, * = uncorrected p < 0.05) towards genes with outlier expression in carrier children (n = 10), carrier parents (n = 6), or noncarrier parents (n = 6). C Forest plot shows classes of “second-hit” variants with significant enrichment (Fisher’s exact test, ** = FDR < 0.05, * = uncorrected p < 0.05) towards genes with outlier expression in carrier children (n = 9) that are shared with either carrier or noncarrier parents. All forest plots show log-odds ratios (dots) and 95% confidence intervals (whiskers). Odds ratios, confidence intervals, p values, and Benjamini-Hochberg corrected FDR values for comparisons with all classes of “second-hit” variants are listed in Additional file 4: Data S2. D Scatter plot shows expression values (transcripts per million, or TPM) for EIF2AK1 in LCL replicates for all individuals (n = 32). Samples in blue have outlier expression of EIF2AK1 (z-score < − 2) and carry a deleterious “second-hit” variant in the 5′ UTR of the gene. E Scatter plots show expression values (TPM) of genes with synergistic effects due to the 16p12.1 deletion and inherited “second-hit” variants. Blue circles indicate expression values for samples from carrier children and family members with rare “second-hit” variants, orange circles indicate expression values for samples from family members without the “second-hit” variant, and green circles indicate expression values of samples from other deletion carriers and noncarriers in the cohort. Black lines denote median gene expression for LCL replicates of each individual used to identify genes with outlier expression in individual deletion carriers

We next investigated whether “second-hit” variants showed synergistic effects towards expression changes in genes also dysregulated by the 16p12.1 deletion. We found 11 instances of genes, such as ANK3, DOCK10, and SLC26A1, that were differentially expressed in all deletion carriers, showed outlier expression in an individual deletion carrier, and had a nearby variant (two coding and nine non-coding) inherited from the noncarrier parent (Fig. 4E; Additional file 1: Fig. S12; Additional file 2: Table S8). For example, two carrier children in family GL_005 inherited an intronic variant within ZEB2 from their noncarrier parent, whose altered dosage is associated with Mowat-Wilson syndrome [92, 93]. While both the 16p12.1 deletion and the “second-hit” variant individually corresponded with increased ZEB2 expression, the presence of both variants in the carrier children resulted in even stronger overexpression of the gene compared to those with either individual variant (Fig. 4E). Overexpression of ZEB2 could contribute to the Mowat-Wilson-like features observed in the carrier child P1C_05, including ID/DD, seizures, hypotonia, and digestive abnormalities. Similarly, a carrier child in GL_005 inherited a rare variant in a promoter region upstream of the mRNA splicing-associated [94] gene SNRNP27 from their noncarrier parent. SNRNP27 is overexpressed in deletion carriers but under-expressed in both the carrier child and the noncarrier parent, highlighting a case where a “second-hit” variant reverses an expression change caused by the deletion (Fig. 4E). Furthermore, a carrier child in GL_004 shared an intronic variant with two noncarrier relatives in the gene SYNJ1, which is associated with synaptic transmission [95] and is under-expressed in carriers of the deletion. While other individuals with the same variant had normal SYNJ1 expression, the carrier child exhibited under-expression of the gene compared to both carriers and noncarriers of the deletion, suggesting that the variant may alter SYNJ1 expression only in the presence of the deletion (Fig. 4E). While it is possible that other variants elsewhere in the genome could also influence expression levels of these genes, these examples highlight putative synergistic effects between the 16p12.1 deletion and “second-hit” variants towards gene expression, where the “second-hit” variants may amplify or reduce the effects of the CNV.

A broad range of transcriptomic alterations contribute to phenotypic variability of the 16p12.1 deletion

To identify a complete spectrum of gene expression alterations in each individual, we next evaluated alternative gene splicing, allele-specific expression (ASE), and expression quantitative trait loci (eQTL) among individuals in our cohort. We first identified an average of 3267 alternative isoforms present in carrier offspring of the 13 trios compared to their parents (Additional file 2: Table S7; Additional file 9: Data S7), including for several neurodevelopmental-associated genes [52] such as KANSL1, SHANK2, and SYNGAP1. After categorizing splicing events by family-specific patterns, we found no differences between splicing events in offspring shared with carrier (average = 1307) or noncarrier parents (average = 1392; p = 0.635, two-tailed paired Mann-Whitney test), with fewer unique changes in the offspring (average = 568; p = 2.44 × 10⁻⁴; Additional file 1: Fig. S13A). We next found enrichments for alternative splicing in genes disrupted by “second-hit” splice-site (p = 7.47 × 10⁻⁴, Fisher’s exact test; FDR = 2.99 × 10⁻³), intronic (p = 9.91 × 10⁻⁹; FDR = 5.95 × 10⁻⁸), or missense SNVs (p = 0.012; FDR = 0.036), interstitial (p = 0.043; FDR = 0.086) and 3′ UTR overhanging deletions (p = 0.024; FDR = 0.058), and intronic STRs (p = 5.75 × 10⁻¹⁰; FDR = 6.90 × 10⁻⁹) (Additional file 1: Fig. S13B; Additional file 7: Data S5). We also found that intronic SNVs were more likely to disrupt splicing in carrier children if they were inherited from the noncarrier parent (p = 0.034, FDR = 0.204) than the carrier parent (Fig. 5A), while intronic SNVs (FDR = 6.36 × 10⁻⁷) and interstitial deletions (FDR = 0.018) were more likely to lead to alternative splicing when present in carrier children than in carrier parents (Additional file 1: Fig. S13C). These results suggest potential correlations between classes of inherited rare variants and alternative splicing events, although changes in isoform expression can only be confidently attributed to rare variants at or near the splice site. For example, a deleterious splice-site variant in the transcriptional activator TADA2A led to an alternate isoform (TADA2A-003) in multiple family members of GL_007 that was not observed in GTEx LCL data [47] (Fig. 5B). TADA2A is a candidate gene within the schizophrenia-associated 17q12 deletion [96], and five out of six family members with the splicing variant have schizophrenia-like clinical features (i.e., hallucinations or delusions), including four deletion carriers and one noncarrier child.

Fig. 5.

Alternative splicing, allele-specific expression, eQTL, and network analysis. A Forest plot shows classes of rare variants with significant enrichment (Fisher’s exact test, ** = FDR < 0.05, * = uncorrected p < 0.05) towards genes with alternative splicing in carrier children (n = 9) that are shared with either carrier or noncarrier parents. Forest plot shows log-odds ratios (dots) and 95% confidence intervals (whiskers). Odds ratios, confidence intervals, p values, and Benjamini-Hochberg-corrected FDR values for comparisons with all classes of “second-hit” variants are listed in Additional file 4: Data S2. B Scatter plot shows isoform usage percentage for TADA2A-003 in replicates for individuals in family GL_007. Samples in blue carry a “second-hit” splice-site variant in TADA2A and exhibit a higher frequency of the alternative isoform. C Scatter plot shows allele frequencies for the autism-associated gene CARD11 in carrier child P2C_07, noncarrier parent F2NC_07, and carrier parent M2C_07 in GL_007. Blue circles indicate allele frequency for haplotypes carrying a “second-hit” coding variant disrupting CARD11. D Scatter plot shows z-scores for expression values of ARHGAP39 for all individuals with available genotypes for the gene. Individuals who carry the minor allele for the ARHGAP39 eQTL (blue dots) have higher expression of the gene than the rest of the cohort (orange dots). E Plot shows correlations among the numbers of gene expression alterations in carrier offspring for the 13 trios assessed in our study. Colors and sizes of the circles are proportional to the correlation coefficients between gene expression changes, where blue indicates a positive correlation and red indicates a negative correlation. Asterisks denote significant correlations (FDR < 0.05, Pearson correlation with Benjamini-Hochberg correction). F Boxplot shows the average shortest distances for carrier offspring (n = 13) between pairs of genes with “second-hit” coding variants and genes with identified expression changes in a brain-specific network. Genes with expression changes were more strongly connected to genes with “second-hit” variants in the brain-specific network than the average distances for genes within 100 permuted brain-specific networks per sample (p = 4.88 × 10⁻⁴, two-tailed paired Mann-Whitney test). Boxplot indicates median (center line), 25th and 75th percentiles (bounds of box), and minimum and maximum (whiskers)

Next, we identified an average of 285 genes with ASE per individual in our cohort (Additional file 2: Table S7; Additional file 10: Data S8), including for the neurodevelopmental-associated genes [52] DNMT3A, NSUN2, and HDAC8. ASE events in the 13 trios were more likely to uniquely occur in the offspring than be shared with a parent (p = 2.44 × 10⁻⁴, two-tailed paired Mann-Whitney test), in contrast to differential expression and alternative splicing events (Additional file 1: Fig. S14A). Genes with ASE have previously been shown to have a higher burden of nearby rare deleterious variants [87], and the pathogenicity of a gene with ASE increases with the presence of a deleterious variant on the overexpressed allele [89]. In our cohort, we found five ASE events in carrier children that led to overexpression of a deleterious “second-hit” coding variant (Additional file 1: Fig. S14B). For example, two carrier children with autism in family GL_007 showed overexpression of a deleterious “second-hit” missense variant in the candidate autism gene [97] CARD11, which was inherited from their noncarrier parent (Fig. 5C).

We further performed eQTL discovery analysis to identify variants statistically correlated with expression changes in our cohort, agnostic to variant pathogenicity or population frequency. We identified 21 eQTLs which modulated the expression of 23 eGenes, or genes whose expression is significantly correlated with an eQTL (Additional file 1: Fig. S15A; Additional file 2: Table S9). Interestingly, 19/21 identified eQTLs were not present in GTEx LCL data [47], representing unique loci in our cohort. Carrier children showed a trend (p = 0.107, two-tailed Mann-Whitney test) towards carrying a higher number of minor eQTLs alleles (average = 4.3/person) than their carrier parents (average = 3.2/person) (Additional file 1: Fig. S15B; Additional file 2: Tables S7, S10). Furthermore, several eGenes had biological functions related to neuronal processes [98–100] (Additional file 2: Table S9), including SERPINF1, BEGAIN, and ARFGEF2. For example, we identified a relatively rare eQTL (allele frequency = 0.015) for overexpression of ARHGAP39, a key regulator of neurogenesis and dendrite morphology associated with learning and memory [101] (Fig. 5D). The eQTL minor allele, located in a transcription factor binding cluster, was only observed in a carrier child and their noncarrier parent within GL_007, who both presented with neuropsychiatric phenotypes.

To assess the joint contributions of each type of expression change among the individuals in our cohort, we assessed correlations between the numbers of gene expression changes assessed in our study by family-specific pattern (Fig. 5E). We observed three significant positive correlations (FDR < 0.05, Pearson correlation) between pairs of gene expression changes in each person, which often shared the same family-specific patterns. Specifically, the number of genes with differential expression strongly correlated with the number of genes with alternative splicing when shared with either the carrier parent (r = 0.93, FDR = 2.91 × 10⁻⁴) or noncarrier parent (r = 0.91, FDR = 4.52 × 10⁻⁴), while unique splicing events in the offspring correlated with splicing events shared with the noncarrier parent (r = 0.83, FDR = 0.011). Together, the correlations between transcriptomic alterations suggest that different types of gene expression changes could co-occur in parents and offspring, potentially due to the same inherited “second-hit” variants disrupting expression of similar genes and biological pathways, as is observed for signals in genome-wide association studies [102].

Genes with “second-hit” variants and expression changes show strong connectivity in a brain-specific network

Finally, to determine whether associations between transcriptomic changes and “second-hit” variants in LCL samples were also relevant in the nervous system, we assessed connectivity patterns of genes with “second-hit” variants and altered gene expression using a brain-specific gene interaction network [75, 76]. We generated individual networks for carrier offspring in the 13 trios and calculated shortest distances between genes with protein-coding “second-hit” variants and genes with LCL-derived expression changes in each offspring (see “Methods”). We found that the average shortest distances between genes with “second-hits” and expression changes were significantly smaller in 6/13 offspring than those derived from permuted networks (FDR < 0.05, one-tailed z-test with n = 100 permutations). In fact, networks for offspring in aggregate had significantly smaller shortest distances (p = 4.88 × 10^-4, two-tailed paired Mann-Whitney test) than the shortest distances from the sets of permuted networks, where genes were randomly reassigned to different nodes in the network (Fig. 5F). These data indicate that “second-hit” variants closely interact with genes with expression changes detected from LCL samples in a brain-specific context, suggesting a potential mechanism for how gene expression changes that underlie developmental phenotypes can be influenced by “second-hit” variants in the genome. However, these findings should be confirmed using expression data from patient-derived neuronal models of the 16p12.1 deletion, as expression changes in LCL samples may not be conserved in the nervous system.

Discussion

We previously described a two-hit model for the 16p12.1 deletion, where the presence of both the deletion and “second-hit” variants determine the phenotypic trajectory of affected children [11, 16]. Here, we propose a potential mechanism for how the deletion and “second-hits” jointly interact to alter clinical phenotypes by way of the transcriptome. We found that the 16p12.1 deletion itself disrupts the expression of genes across the genome through direct effects, such as chromatin interactions, and through indirect effects, such as downstream genetic interactions (Fig. 6). For example, chromatin interactions were observed between regions within the 16p12.1 deletion and flanking genes such as STX1B and DNAH3, and 1493 genes outside of chromosome 16 were also dysregulated in deletion carriers. The identification of flanking genes downregulated by the deletion is in line with similar findings for the 16p11.2, 1q21.1, and 22q11.2 deletion disorders [21, 103]. Each of these CNVs exhibited altered gene expression in adjacent regions that is putatively mediated by chromatin interactions, highlighting the importance of considering the three-dimensional structure of the genome to elucidate CNV pathogenicity. Similarly, we found that “second-hits” disrupt gene expression through both direct and indirect mechanisms. Genes with nearby “second-hit” variants were more likely to exhibit outlier expression and alternative splicing, and genes with “second-hits” were more closely connected to genes with expression changes in a brain-specific network than random sets of genes in permuted networks. In fact, we observed 11 examples of combined effects of the deletion and “second-hit” variants towards expression in our cohort, including the candidate neurodevelopmental genes SYNJ1 and ZEB2. These synergistic effects towards gene expression are similar to those previously observed for eQTLs [104] and HLA alleles [105], except that these effects are potentially due to the combined effects of rare deleterious variants. We note that only a subset (~11%) of genes with altered expression in our cohort harbored deleterious “second-hit” variants that could affect expression. It is likely that the downstream effects of both the deletion and “second-hit” variants could be responsible for a larger proportion of gene expression changes, along with other common variants and environmental factors. Thus, our results suggest that the 16p12.1 deletion and the “second-hit” variants interact with each other in a complex manner to mold the shape of the transcriptome, resulting in strong dysregulation of developmental genes and contributing to neuropsychiatric features in 16p12.1 deletion carriers.

Fig. 6.

Genetic and transcriptomic mechanisms for phenotypic variability in 16p12.1 deletion families. Affected children inherit the 16p12.1 deletion (red) and a smaller number of rare “second-hit” variants (green) from a carrier parent, and a larger number of “second-hit” variants from the noncarrier parent (blue). Altered expression of genes due to these “second-hit” variants affects nearby downstream connected genes in an interaction network (grey), causing additional transcriptomic perturbation. Because of this, carrier children have numerous gene expression changes compared with their carrier parents, including genes showing synergistic effects of the deletion and “second-hit” variants (orange), potentially accounting for more severe developmental phenotypes observed in the children

Results from our study align with previous studies, which found that rare variants of different classes have varying effect sizes towards gene expression [25, 87]. Our study extends this paradigm by identifying classes of rare “second-hit” variants whose contributions to gene expression changes differ by inheritance pattern. We found that high-effect variants, such as whole-gene duplications, cause expression changes regardless of parent-of-origin, and splice-site variants lead to changes in isoform expression independently of inheritance. In contrast, lower-effect variants, including missense, silencer, and upstream SNVs, were more strongly associated with gene expression changes when inherited from the noncarrier parent than the carrier parent. These findings indicate that noncarrier parents are more likely to pass gene expression-altering “second-hit” variants down to their carrier children, potentially accounting for more severe phenotypic manifestations in children with the deletion compared with their carrier parents (Fig. 6). One potential explanation for why carrier children receive a higher number of deleterious variants from their noncarrier parent is assortative mating among their parents, as 8/8 carrier parents and 7/9 noncarrier parents in our cohort manifested at least mild neuropsychiatric features. Assortative mating has been extensively observed among individuals with neurodevelopmental or psychiatric disorders [106, 107], in particular autism [108], suggesting its relevance towards phenotypic variability among deletion carriers in our cohort. Future family-based transcriptome studies with larger sample sizes may be able to pinpoint specific rare variants within dysregulated genes that are associated with distinct phenotypes in the carrier children.

We also identified putative biological and developmental pathways disrupted by both the deletion and “second-hit” variants. For example, we found that genes differentially expressed by the deletion were preferentially expressed in multiple brain tissues during development and were enriched for core signaling and developmental pathways. In fact, knockdown of individual homologs of 16p12.1 genes in Drosophila melanogaster models showed neuronal phenotypes and transcriptome disruptions, suggesting that the individual effects of multiple genes in the deletion sensitize the genome for neuropsychiatric phenotypes [109]. Interestingly, we found several examples of biological functions and mechanisms that were simultaneously dysregulated by both the deletion and “second-hit” variants in the carrier children. For example, most carrier children shared differential expression in genes enriched for nervous system development, cell adhesion, signaling, and locomotion with both their carrier and noncarrier parents. These results provide insights into how the deletion and “second-hit” variants synergistically dysregulate genes and pathways related to development, ultimately contributing towards a wide range of developmental phenotypes observed in children with the deletion.

Some limitations can be noted in the context of our study. First, we investigated gene expression changes within patient-derived LCL samples, which have reduced relevance for brain expression. However, over 80% of genes expressed in GTEx brain samples, as well as over 70% of neurodevelopmental disease genes, were expressed in our LCL samples (Additional file 1: Fig. S4A-B). Nevertheless, repeating the study in tissues that are implicated in neurodevelopmental disorders, potentially using patient-derived reprogrammed neuronal progenitor cells, would verify the associations between variants, expression changes, biological functions, and clinical features. Second, we have a relatively small cohort of 32 individuals within five families. It would be useful to determine whether the identified associations are strengthened in a larger cohort, especially those that did not pass multiple-testing corrections. Phenotypically more diverse cohorts would also allow for performing additional correlations between gene expression changes and specific clinical features, such as whether more outlier genes are present among families with stronger histories of neuropsychiatric disease.

Conclusions

Overall, our work supports a model for complex disorders, where combinatorial effects of multiple variants with different effect sizes affect expression of genes in developmental pathways, which further influence the expressivity of clinical features. These results exemplify that family-based transcriptome studies, similar to family-based genome studies, can help explain changes in phenotypes from parents to children and between siblings, especially in complex disorders with a high degree of intra- and inter-familial variability.

Abbreviations

ASE

Allele-specific expression

CNV

Copy-number variant

ID/DD

Intellectual disability/developmental delay

LCL

Lymphoblastoid cell line

LOF

Loss-of-function

LOF

Loss-of-function

PAGE

Parametric analysis of gene set enrichment

RIN

RNA integrity number

SNV

Single-nucleotide variant

STR

Short tandem repeat

TPM

Transcripts per million

TSS

Transcription start site

UTR

Untranslated region

WGCNA

Weighted gene correlation network analysis

WGS

Whole-genome sequencing

Authors’ contributions

MJ, AT, and SG conceived the project. MJ and AT performed all analyses in the manuscript, generated the plots and images, and wrote and revised the manuscript. LP recruited the families, obtained and assessed clinical phenotypes, and isolated DNA and RNA for sequencing. CS assisted with collection of patient clinical information and bioinformatic pipelines to identify WGS variants. MD assisted with extraction of RNA from LCL samples. EH assisted with collection of patient clinical information. AK provided the brain-specific network and assisted with the network and WGCNA analyses. SG supervised the research, recruited the families, assisted with collection of patient clinical information, and wrote and revised the manuscript. All authors read and approved the final draft of the manuscript.

Funding

This work was supported by NIH R01-GM121907 and resources from the Huck Institutes of the Life Sciences to S.G. M.J. was supported by NIH T32-GM102057. A.T. was supported by NIH T32-LM012415. L.P. was supported by Fulbright Commission Uruguay-ANII. A.K. was supported by NIH R35-GM128765. The funding bodies had no role in the design of the study, the collection, analysis, and interpretation of data, or in writing the manuscript.

Availability of data and materials

Patient-derived LCL samples generated in this study are available at the NIGMS Human Genetic Cell Repository at the Coriell Institute (https://www.coriell.org/1/NIGMS). Accession numbers for LCL samples are provided in Additional file 2: Table S5. Whole-genome sequencing, SNP microarray, and RNA sequencing data generated in this study are available at NCBI dbGaP study accession phs002450 (http://www.ncbi.nlm.nih.gov/projects/gap/cgi-bin/study.cgi?study_id=phs002450.v1.p1) and BioProject accession number PRJNA734670 [30]. All other data generated or analyzed during this study are included in this article and its supplementary information files. All code generated for this project, including pipelines for running bioinformatic software and custom analysis scripts, are available at https://github.com/girirajanlab/16p12_RNAseq_project [110] and https://github.com/girirajanlab/16p12_WGS_project [111].

Declarations

Ethics approval and consent to participate

Carrier children and their family members provided informed consent according to a protocol reviewed and approved by the Pennsylvania State University Institutional Review Board (IRB #STUDY00000278). All research in this study conformed to the principles of the Helsinki Declaration.

Consent for publication

Written informed consent for publication of clinical details was obtained from all participants, including legal guardians of affected children.

Competing interests

The authors declare that they have no competing interests.