Contactins and Contactin-Associated Proteins, and Contactin-Associated Protein-Like 2 (CNTNAP2) in particular, have been widely cited as autism risk genes based on findings from homozygosity mapping, molecular cytogenetics, copy number variation analyses, and both common and rare single nucleotide association studies. However, data specifically with regard to the contribution of heterozygous single nucleotide variants (SNVs) have been inconsistent. In an effort to clarify the role of rare point mutations in CNTNAP2 and related gene families, we have conducted targeted next-generation sequencing and evaluated existing sequence data in cohorts totaling 2704 cases and 2747 controls. We find no evidence for statistically significant association of rare heterozygous mutations in any of the CNTN or CNTNAP genes, including CNTNAP2, placing marked limits on the scale of their plausible contribution to risk.
Citation: Murdoch JD, Gupta AR, Sanders SJ, Walker MF, Keaney J, Fernandez TV, et al. (2015) No Evidence for Association of Autism with Rare Heterozygous Point Mutations in Contactin-Associated Protein-Like 2 (CNTNAP2), or in Other Contactin-Associated Proteins or Contactins. PLoS Genet 11(1): e1004852. https://doi.org/10.1371/journal.pgen.1004852
Editor: Jonathan Flint, The Wellcome Trust Centre for Human Genetics, University of Oxford, UNITED KINGDOM
Received: May 28, 2014; Accepted: October 26, 2014; Published: January 26, 2015
Copyright: © 2015 Murdoch et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited
Data Availability: All raw data are publicly available at the NDAR website (https://ndar.nih.gov/data_from_labs.html) under the heading "Genomic Profiling and Functional Mutation Analysis in Autism Spectrum Disorders" and accession #1895. Approved researchers can obtain the SSC biospecimens described in this study (http://sfari.org/resources/simons-simplex-collection) by applying at https://base.sfari.org and completing the Researcher Distribution Agreement which ensures these are being used for appropriate scientific purposes. The Baylor-Broad data are from the “Analysis of rare, exonic variation amongst subjects with autism spectrum disorders and population controls” study (PMID 23593035), whose authors may be contacted at email@example.com and firstname.lastname@example.org.
Funding: This work was supported by grants R01 MH081754 and RC2 MH089956 to MWS, and by K08MH087639 to ARG. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Contactin-associated protein-like 2 (CNTNAP2; a.k.a CASPR2, OMIM 604569, Swiss-Prot Q9UHC6), is widely considered an established autism spectrum disorder (ASD, OMIM 209850) risk gene based on a series of findings including homozygosity mapping of rare recessive mutations, cytogenetics[2, 3], deep re-sequencing, common variant candidate gene association studies[3, 4], and behavioral phenotyping of mouse models. Moreover, several of the reported human genetic studies have extended the linked or associated phenotype to include language delay[6, 7], intractable epilepsy, cortical malformation and intellectual disability[8, 9] (OMIM 610042) and in one instance, hepatomegaly and periventricular leukomalacia. These findings, in aggregate, point to an important role for CNTNAP2 in the development of the human central nervous system and provide strong evidence that the complete loss of function of this protein leads to autism and epilepsy. However, replication of the genetic association studies with regard to heterozygous variants in ASD2–4 has proven elusive. With regard to common variation, three genome wide association studies have not found further significant evidence for previously identified single nucleotide polymorphisms (SNPs)[11–13] at CNTNAP2 while a fourth found suggestive evidence falling short of genome-wide significance for a nearby SNP. Moreover, a recent targeted study of common alleles at the CNTNAP2 locus did not replicate prior findings or provide new evidence for significant associations in this interval, after correction for multiple comparisons and the inclusion of a larger follow-up cohort.. In addition, to our knowledge, there have been no further published investigations of rare variant mutation burden in CNTNAP2 beyond the initial report from our laboratory.
In an effort to further explore the evidence for a role for rare heterozygous mutations in CNTNAP2 in ASD, we set out to re-sequence a new discovery cohort including 1030 individuals affected with ASD as well as 942 psychiatrically unscreened controls, using a combination of micro-emulsion PCR and next generation sequencing. Moreover, we extended our investigation to include the additional genes Contactins 1–6 (OMIM 600016, 190197, 601325, 607280, 607219, 607220, respectively; Swiss-Prot Q12860, Q02246, Q9P232, Q8IWV2, O94779, Q9UQ52, respectively) and Contactin Associated Proteins 1, 3, 4 and 5 (OMIM 602346, 610517, 610518, 610519, respectively; Swiss-Prot P78357, Q9UHC6, Q9BZ76, Q9C0A0, Q8WYK1, respectively), based on a range of evidence for several of these neuronal adhesion molecules in neurodevelopmental phenotypes[16–18].
In our prior analysis of CNTNAP2, sequencing of a separate cohort of 635 cases and 942 controls led to the identification of one nominally significant rare variant, I869T, found in three apparently unrelated cases and not in controls, though at the time of publication we were not able to rule out a role for population stratification in this finding. In addition, we observed an approximately 2 fold increase in rare highly conserved (across 10 vertebrate lineages) mutations in cases versus controls, but this fell just short of statistical significance. In the current study, after correction for multiple comparisons, we find no additional support for an association of the I869T variant, which in contrast to our prior study, is no longer predicted to be deleterious to protein function [19, 20]. Morevoer, we find no evidence for association of rare heterozygous mutations in general in CNTNAP2 with the ASD phenotype, either in our new discovery cohort (N = 1030 cases and 942 controls), among an independent ASD sample that had previously undergone exome sequencing (N = 1039 ASD cases and 863 controls), or in a combined mutation burden analysis including these two data sets along with the cohort previously sequenced in our laboratory (N = 2704 cases and 2747 controls). Our ability to assess the impact of rare loss of function mutations was limited by very few observations. However, our findings with regard to rare missense variants was not altered by predicting putative functional versus neutral variants using a range of informatics tools. Finally, we found no significant support for association of rare heterozygous mutations in other Contactins or Contactin-Associated Proteins via targeted re-sequencing of our discovery cohort (1030 cases and 942 controls).
Given the strong evidence for a link between ASD, epilepsy and homozygous loss of CNTNAP2, our data do not rule out a role for this gene and associated molecules in the risk for ASD, but place further bounds on the plausible size of the contribution from rare heterozygous missense mutations in these genes.
Burden of rare mutations in cases and controls
In prior work we had noted a non-significant overrepresentation of all rare (<1 observation in 4000 combined [sequenced or TaqMan-genotyped] controls) variants in affected individuals. Consequently, our primary hypothesis was that in an expanded analysis, the burden of rare mutations would be greater in cases than in well-matched controls. After QC steps and exclusion of ancestral outliers, we had a total of 1030 cases and 942 controls and conducted a gene by gene analysis, including variants that were missense, nonsense, or splice site-disrupting, fell below 2% in the high-throughput data, and were filtered against population data as described in Methods below. Variants that were present only once in cases or controls are denoted as “singleton” and are estimated to have an allele frequency approximate to that in our prior analysis (<1 observation/4000). For CNTNAP2, we found no increase in the overall burden of rare mutations (Table 1, Fig. 1) even before correcting for multiple comparisons and in fact more rare mutations in controls than cases (19 in cases, 26 in controls, Fisher exact one-tailed p = 0.113). We then evaluated all CNTN and CNTNAP genes and nominal association for rare heterozygous mutations in CNTN1 (14 in cases, 5 in controls, Fisher exact one-tailed p = 0.048) and CNTN3 (13 in cases, 3 in controls, Fisher exact one-tailed p = 0.016), however, neither results survived experiment-wide correction for multiple comparisons.
Mutations were counted if missense, nonsense, splice site, or frameshift in CNTNAP2 (in point of fact, all were missense). Variants in red are exclusive to cases; those in green, controls. Those predicted to be deleterious in SIFT are underlined in orange; in PolyPhen2, purple. Domain names and approximate locations from Bakkaloglu et al.,
We reasoned that the background rate of neutral rare variation in the genome might be obscuring a true difference in functional alleles in cases versus controls. Consequently, we used a variety of defining criteria to try to distinguish the subset of potentially disease-relevant mutations: First, we evaluated “singleton” mutations, i.e. those seen only once either in cases or in controls. This strategy was intended to focus on the rarest alleles in our sample, those most likely to be subject to purifying selection. A comparison of rates of singleton mutations in CNTNAP2 and all other sequenced CNTN and CNTNAP genes again found no evidence of association, prior to correction for the 10 genes evaluated in this study (Table 2). We then used two well-established informatics tools designed to predict deleterious amino acid substitutions. PolyPhen2 and SIFT , . We defined mutations as deleterious if they were either ‘possibly damaging’ or ‘probably damaging’ in PolyPhen2 or ‘damaging’ in SIFT. While neither metric evaluates nonsense mutations and splice site disruptions, these were included as deleterious as well.
Using all of these approaches separately, we compared the rates of putatively deleterious/functional alleles in the same 1030 cases versus 942 controls. We found no significant differences using any of these metrics with regard to CNTNAP2 (13 in cases, 13 in controls, Fisher exact one-tailed p = 0.486) (Table 3). CNTN1 was found to show nominally significant association (12 in cases, 2 in controls, Fisher exact one-tailed p = 0.01) but this was not significant after correcting for the 10 genes studied. No other genes were significant prior to correction. Additionally, in an analysis restricted to singletons predicted to be deleterious by SIFT or PolyPhen2 (S1 Table), none of the genes reached significance prior to correction.
Finally, we restricted our analysis to focus solely on nonsense, splice site or frameshift mutations. We found none present in CNTNAP2 in the current cohort. Moreover, this category of variation was so infrequent in both cases and controls in all other genes investigated that gene-by-gene analysis was not statistically meaningful, this limiting our conclustions about the role for true haploinsufficiency in any of the genes under study. Overall, we found 2 case individuals with a stop codon in one of the 10 genes (CNTN2 and CNTNAP1), 1 case and no controls with a splice site mutation (CNTN3), and 3 control individuals displaying a stop codon (CNTNAP1 and two in CNTN6). Of note, indel mutations were not detectable using the Raindance instrument given the short read length and the nature of the alignment process.
Of note, our primary analysis was restricted to only rare variants seen in cases or controls and not both. To be confident that this approach did not obscure a true difference in mutation burden, we re-ran all of the aforementioned analyses while including all point mutations defined as rare, regardless of whether they were present in both cases and controls. This had no impact on the interpretation of our results (S2‐S3 Tables).
Power of burden test
For the primary analysis of CNTNAP2, we compute good power (>80%) under the following parameters: observed rare variant frequency of 0.023 (Table 1), odds ratio for dominant effect of ≥ 2.0, size of the test set to 0.005 (corrected for 10 tests), and for this sample of cases (N = 1030) and controls (N = 942). The empirically derived rare variant frequency for the average gene tested is lower (across all CNTNs and CNTNAPs including CNTNAP2) at 0.015. For such a gene, good power accrues for odds ratio ≥ 2.5. Finally, it we consider the burden over all tested genes combined, for which the average frequency of rare variants is roughly 0.15, good power accrues if the odds ratio is ≥ 1.35.
Analysis of I869T
In our 2008 report, we regarded I869T as a significant finding given its occurrence 3 times in cases and not at all in controls (Fisher exact one-tailed p = 0.014), its deleterious rating in SIFT, and its amino acid conservation [leucine in amphibians and fish, isoleucine in mammals]. Subsequent revisions to SIFT, however, have reclassified the mutation as benign, and its PolyPhen2 rating has remained benign. Furthermore, the expanded omnibus data set of 2704 cases and 2747 controls (S4 Table) revealed just one further occurrence in cases (in the Broad-Baylor cohort), none in controls; this was no longer statistically significant in the expanded sample size (Fisher exact p = 0.06) without correction for multiple comparisons.
De Novo mutation burden
In keeping with our recent findings that the identification of recurrent de novo loss-of-function point mutations is a viable strategy to identify ASD genes, we determined the transmission status of every rare/singleton mutation seen in probands. We found 2 confirmed de novo mutations using whole blood DNA for sequencing reactions. No confirmed de novo mutations were observed in CNTNAP2. CNTN6 and CNTNAP4 each showed one de novo missense variant each. Based on recent analyses of exome data, a single missense de novo mutation, regardless of other characteristics such as degree of evolutionary conservation, does not provide significant evidence of association.[23–26]
Compound heterozygous mutations
We further examined individuals for the presence of multiple rare variants in the same gene: We found 2 probands with rare mutations, one in CNTN6 and the other in CNTNAP4. A total of four controls were also identified with two rare mutations each: three were found in CNTN5, and one had two rare variants in CNTN6. We determined chromosome phase for the two cases and both were found to be compound heterozygotes. A similar analysis was not possible for controls given the absence of parental data. Again, based on recent studies of whole-exome trio data in autism, the observation of a lone missense compound heterozygous mutation in a gene carries minimal statistical evidence for association.
Parental origin of mutation
With the family analysis data, we were able to determine inheritance status (S5 Table) for putatively deleterious mutations of interest in each gene. There was no significant difference in the proportion of deleterious (based on ratings in SIFT (damaging) and/or PolyPhen2 (possibly or probably damaging) variants maternally inherited and paternally inherited in any gene (Table 4). We also observed no significant difference between maternal and paternal variants when this gene-by-gene analysis was restricted to singletons (S6 Table).
Combined analysis of multiple cohorts for mutations in CNTNAP2
Given the divergent findings in our initial study versus the new discovery cohort with regard to CNTNAP2, we expanded our dataset. Using exome sequencing data in both cases and controls, we were able to increase the total sample for this gene to 2704 cases and 2747 controls. Consistent with the findings above, an omnibus analysis in these 2704 cases and 2747 controls showed no significant results either in a primary analysis of rare mutation burden or in any of the exploratory analyses of variant subsets, as described above (rare mutation burden 45 in cases, 49 in controls, one-tailed Fisher exact p = 0.407, deleterious mutation burden 26 in cases, 28 in controls, one-tailed Fisher exact p = 0.469, deleterious singleton mutation burden 22 in cases, 23 in controls, one-tailed Fisher exact p = 0.521) (Tables 5, S7 and S8). Furthermore, the variants from our 2008 paper show an even weaker trend for overrepresentation of deleterious mutations in cases, due to updates to the SIFT and PolyPhen2 databases (see Tables 5, S7 and S8).
Strauss et al. first demonstrated a role for CNTNAP2 in neurodevelopmental disorders based on a consanguineous pedigree in which probands presented with autism, cortical dysplasia and focal epilepsy. A single-base homozygous deletion resulting in a premature stop codon was identified in CNTNAP2. In 2008, four studies provided varying degrees of evidence for a role for heterozygous mutations in CNTNAP2 in non-syndromic autism and language delay. Bakkaloglu et al. mapped a de novo chromosomal inversion disrupting CNTNAP2 and then re-sequenced the gene in 635 cases and 942 controls, finding nominally significant association of a single rare variant and a trend toward significance for the overall burden of rare deleterious and conserved mutations in cases versus controls. Alarcon et al. utilized family-based association with age at first word in 172 autism trios to identify CNTNAP2 along with three other genes; in a second-stage follow-up in 304 independent trios, only CNTNAP2 continued to show association with age at first word. Furthermore, microarray expression analysis identified 12 genes significantly enriched in human language-related association cortex, one of which was CNTNAP2. Arking et al. used a linkage approach and identified a common variant in CNTNAP2; a second-stage independent cohort of 1295 autism trios showed significant overtransmission of the T allele. Finally, Vernes et al., investigating the transcription factor FOXP2, previously implicated in language disorders[28–30], determined that FOXP2 binds to and downregulates CNTNAP2. Additional case reports of speech delay and/or ASD patients demonstrating disrupted CNTNAP2 have subsequently been identified[7, 31]. Most recently, Peñagarikano reported a CNTNAP2 KO mouse that showed deficiencies in all three ASD core behavioral domains, seizures, and hyperactivity, with demonstrable neuronal migration aberrations, abnormal cellular morphology and a deceased number of interneurons.
Additionally, disruptions in other members of the contactin family and contactin-associated protein-like family have also been associated with autistic phenotypes. Multiple case reports have implicated contactin 4 (CNTN4) in ASD and in developmental delay[17, 32], as did a CNV study described above. Contactin-associated protein-like 5 has also been recently implicated in ASD by a case study .
However, subsequent to these reports, the evidence for association of heterozygous variants in CNTNAP2 has been variable. As noted, multiple GWAS analyses[11–13] have not identified evidence of genome-wide significant association of SNPs mapping near CNTNAP2. In addition, to date, neither rare de novo [23–26] or compound heterozygous mutations[27, 34, 35] have implicated CNTNAP2 or other Contactin or Contactin Associated Proteins in autism or related phenotypes. Finally, other CNTN genes have so far not been subjected to large-scale case control rare variant analyses.
Against this backdrop, we undertook a follow-up of our earlier rare variant case control analysis focusing on CNTNAP2, and expanded the study to include other CNTN and CNTNAP genes. As described above, our results do not convincingly replicate association of the previously nominally significant variant, I869T, nor support the association of heterozygous rare mutations, either transmitted or de novo, in CNTNAP2 with the ASD phenotype. Nor is there evidence for rare recessive risk alleles in this outbred cohort. We found similar results for all CNTN and CNTNAP genes tested here. As noted above, in addition to investigating overall mutation burden, we conducted exploratory analyses to look for any potential differences between cases and controls in subsets of patients; these included evaluating predicted deleterious mutation burden, looking for multiple mutations within a single gene or across the genes sequenced in this study (see Protocol S1), investigating parental origin of the variation and evaluating for de novo mutations. While the primary analyses were well-powered to identify odds ratios in the range of 1.35 to 2.5, the secondary analyses are truly exploratory and cannot be interpreted as excluding a role for CNTN or CNTNAP genes in ASD.
There are several potential explanations for our inability to extend our previous findings: first, the prior results with regard to overall mutation burdent showed only a trend toward signigficance and the larger, better powered sample studied here may simply be clarifying the true relationship (or absence of risk). Alternatively, the paucity of loss of function mutations in the expanded sample, coupled with the difficulty in interpreting the functional consequences of transmitted missense variants without a biologically validated assay could now be leading to a false negative result with regard to haploinsufficiency at this locus—though our results do strongly suggest that the overall contribution to population risk of heterozygous mutations of all types in CNTN and CNTNAP2 must be quite limited. With regard to the prior finding of association of the I869T variant in cases, we did not find evidence for population stratification playing a role, but neither did we add substantial evidence for association, again limiting the plausible effect size of this risk.
As noted above, the lack of a reliable functional assay allowing us to differentiate biologically meaningful from neutral variants is an important limitation of the study. It is possible that such an assay could reveal a distribution of variation consistent with an effect for heterozygous mutations in CNTNAP2—or any of the other genes we have studied. Similarly, it was notable that we did not observe any putative loss of function mutations (nonsense, frame-shift, splice site) in either cases or controls for CNTNAP2. Given the finding of a severe neurodevelopmental syndrome resulting from homozygous loss of function mutations, the observation of deletion CNVs at this locus in affected individuals, and the absence of clear LOF mutations in our sample, it remains possible that very rare LOF heterozygous mutations in CNTNAP2 carry some risk for ASD. Nonetheless, based on the current study, our results place limits on the degree to which, overall, rare heterozygous missense mutations in Contactin and Contactin Associated Proteins may play a role in the population risk for ASD.
They similarly suggest that it is not yet possible to determine the clinical significance of individual rare heterozygous mutations in CNTNAP2, identified either in a research cohort or in diagnostic assays (http://www.athenadiagnostics.com/content/test-catalog/find-test/service-detail/q/id/1487).
Materials and Methods
Subjects and experimental structure
For the targeted re-sequencing discovery cohort, 1332 ASD probands were obtained from the Simons Simplex Collection (SSC), a cohort focused on simplex autism families. Only probands from the SSC were sequenced. We elected to compare this cohort to 1015 unrelated controls, determined to be neurologically unaffected, drawn from the NINDS Caucasian controls repository (Coriell, Camden, NJ). As described above and in detail in Protocol S1, the final case-control cohort was filtered to 1030 ASD probands and 942 controls. For the follow-up examination of CNTNAP2, we obtained exome sequencing data from the ARRA Autism Sequencing Collaboration (AASC). AASC cases and controls were genotyped on the Illumina 550K Single BeadChip platform and filtered to exclude any individual with a genotyping call rate <95%, discrepant genotype data with regard to reported sex, Mendelian inconsistencies, or cryptic relatedness, resulting in a final sample of 1039 autism cases and 863 controls, all of whom were determined to be of European descent through ancestry matching via PCA of genotyping data. Controls were screened for psychiatric conditions via questionnaire. Although AASC/ARRA variants were not confirmed via Sanger sequencing as the Yale cohort of 1030 cases and 942 controls were, we concluded that given the identical sequencing methods for cases and controls as well as the approximately equal sample sizes, any errors would be reasonably randomly distributed among cases and controls. Sample characteristics and diagnostic methodology for the AASC have been described previously.5 This study was approved by the Institutional Review Boards of both Yale University and the Broad Institute.
Primer emulsions representing 1152 separate amplicons were designed and synthesized by Raindance Technologies (Lexington, MA). Synthesis was infeasible for much of CNTNAP3 due to highly repetitive regions; because 16 exons out of 24 were excluded, this gene was not sequenced and therefore does not contribute to any further analyses. A single exon was omitted from each of the genes CNTN2 (out of 22 exons total) and CNTNAP4 (25 total) each due to difficulty in primer synthesis. We reasoned that any loss of data should be equally distributed across cases and controls.
In the initial sequencing effort, all DNA used was derived from human lymphoblastoid cell line DNA. All confirmations, however, were conducted in DNA derived from blood (see below). Samples were quantified on a Biotek Synergy HT fluorometer (BioTek US, Winooski, VT). After quantification, DNA was pooled, 8 individuals at a time, by case/control status (Protocol S1).
Pooled DNA samples were sheared on a Covaris S2 (Covaris, Inc., Woburn, MA) to an approximate size of 3 kb and combined with RainDance microemulsion PCR master mix prepared according to the protocol, then run with a standard protocol on the RDT1000 machine (Raindance Technologies, Lexington, MA) and subjected to conventional PCR on a thermal cycler.
After successful droplet merging and PCR, the samples were cleaned according to the RainDance protocol; aqueous PCR product phase was purified on Qiagen MinElute columns (Qiagen GmbH, Hilden, Germany) and run on an Agilent Bioanalyzer according to DNA1000 protocol. Product was then blunted and concatenated into longer DNA fragments, because the range of amplicon sizes in the microemulsion library makes sequencing uniform fragment lengths impossible without first concatenation and subsequent shearing.
Concatenated DNA was sheared on a Covaris S2 to a mean size of 200 bp. Products were processed for end repair, adenylation and adapter ligation according to modified Illumina protocol (S1 Protocol). These fragments were size selected on Invitrogen agarose e-gels (Invitrogen, Life Technologies, Carlsbad, CA); size-selected DNA fragments were enriched using Illumina primers InPE 1.0, InPE 2.0, and a selected Illumina barcode index out of 12 available. Barcode indices were selected as described in Protocol S1. PCR was performed according to standard Illumina multiplexing protocol and samples were cleaned up on MinElute columns; this product was then re-purified on an e-gel to remove primer dimer and all non-product fragments from the amplified product. 1 µL of this product was run on an Agilent 2100 Bioanalyzer according to DNA1000 protocol to quantitate final concentration.
Sequencing of the discovery cohort
Separate pools of 8 case and 8 control samples were mixed in a 1:1 equimolar ratio and sequenced on the Illumina Genome Analyzer IIx. Sequence reads were run through a data analysis pipeline on a high performance cluster (HPC) and aligned to the human genome (NCBI build 36, hg18) using the aligner BWA, followed by conversion to SAM format and generation of a Pileup file using SAMtools. The Pileup file was then analyzed and annotated to identify variants with a haploid coverage greater than 80X, minor allele frequency (MAF) greater than 3.5% and a PHRED-like score (generated from the quality scores in the initial reads) greater than 20. The MAF and Phred-like score cutoffs were determined empirically. Annotation was performed for all possible isoforms of each gene to ensure that any deleterious variants were detected.
Pools in which putative rare mutations of interest were identified underwent confirmation and deconvolution using Sanger sequencing. Mutations of interest were defined as missense, nonsense, splice site, or start or stop codon disruptions with a frequency of less than 2%, and less than 1% in all populations in the Exome Variant Server and SeattleSNP databases. Only a single region showed repeated PCR failures (chr11:99437155, CNTN5). This variant was excluded from any further analyses. The confirmation rate of the high-throughput sequence variant predictions of interest, as determined from all variants which successfully underwent PCR and Sanger sequencing, was 92%.
After successful Sanger confirmations, all variants identified only in cases were tested for de novo status. An initial round of re-sequencing of the proband, parents and any siblings was completed using lymphoblastoid DNA; if the mutation appeared to be de novo, a second round of sequencing in all family members was completed using whole blood DNA to rule out false positives resulting from EBV transformation. Family member DNA was not available for inheritance evaluation in the Coriell controls.
As part of our analytic strategy we planned to evaluate de novo mutations, and consequently we required a high level of certainty regarding the identity of any proband carrying a putative mutation. Consequently, we developed an in-house script to verify pool composition by comparing returned pooled next-generation sequence data to previously obtained genotyping data available on all SSC probands reported here. 15 pools (9 cases and 6 control) demonstrated insoluble identity issues (ambiguity of constituent individuals) and were excluded from all analyses.
Sample quality control and adjustments for comparable ancestry
SNP Genotyping was performed on Illumina 1M arrays at the Yale Center for Genome Analysis using whole blood DNA (SSC samples) or lymphoblastoid cell line DNA (NINDS controls). Redundant samples were removed from both the case and control cohorts. After sample removal, 1266 cases and 1015 controls genotyped concurrent with being run on Raindance. Of these, PLINK was used to remove those with missing genotype data or call rates <95%, to remove inconsistencies in reported sex, to detect and remove Mendelian inconsistencies, and to identify and remove cryptically related samples using an assessment of inheritance by descent up to and including 2° relatives—after all other filtering steps, one proband was excluded due to relatedness.
Principal components analysis was performed with the genotype data from these samples using Golden Helix SNP and Variation Suite v7.5.4 (Bozeman, MT, USA), evaluating 8210 tagging SNPs SNPs not found to be in high linkage disequilibrium, used in the same way as described in a recent paper. Based on a scree plot, we plotted the eigenvalues of the first 3 principal components which accounted for 32%, 23% and 11% of variation. We defined the final NINDS control set of 942 as a Caucasian cohort and observed that a threshold of 5 interquartile ranges from the third quartile contained all NINDS controls; we used this criterion as a cutoff. 50 SSC probands lay outside this threshold at 6 IQR or greater and consequently were excluded from further analysis.
The Baylor-Broad ARRA set consisting of 1039 cases and 863 controls was used to follow-up on our targeted sequencing data given its comparable size and ancestry-matched selection of probands.
All statistical tests were one-tailed Fisher exact tests, with the exception of parent-of-origin analysis (see below). We used a Bonferroni correction by a factor of 10, based on the 10 genes investigated. Any variant that was seen in both cases and controls was excluded from the analysis. Because parent of origin was a binomial outcome, per-gene one-tailed binomial tests were performed. Finally, in the combined CNTNAP2 dataset of our 2008 data, the current data, and the Baylor-Broad ARRA data, any variants seen in cases and controls were removed from the set (resulting in the loss of one variant from the cumulative set.)
S1 Protocol. Details of DNA quantitation, shearing, Raindance and PCR conditions, Illumina sequencing preparation, post-sequencing bioinformatics methods, and variant counting.
S1 Table. The deleterious singleton mutation burden as defined by a rating of “damaging” in SIFT and/or “possibly damaging” or “probably damaging” in PolyPhen2.
S2 Table. Rare mutation burden including variants seen in both cases and controls as well as those exclusive to cases or controls.
S3 Table. Rare deleterious mutation burden including variants seen in both cases and controls as well as those exclusive to cases or controls.
S4 Table. The individual mutations in CNTNAP2 in cases and controls in this discovery set, the 2008 data as reported in Bakkaloglu et al., and the Baylor-Broad data.
S5 Table. Parent of origin of all inherited mutations in all genes, with deleterious status indicated.
S6 Table. The inheritance patterns at all genes of singleton mutations regarded as deleterious.
S7 Table. Overall rare mutation burden in CNTNAP2 in cases and controls in this discovery set, the 2008 data as reported in Bakkaloglu et al., and the Baylor-Broad data.
We are grateful for the contributions of the management and staff at at the Yale Center for Genomic Analysis, particularly Shrikant Mane, Milind Mahajan, Irina Tikhonova, Joshua Lubner, Kira Fitzsimons, David Harrison, Anna Rogers, Nicole Pizzoferrato, and Vanessa Spotlow, and to Nicole Wright, Sindhuja Kammela, and Jaclyn Jacobi for technical support. We thank T. Brooks-Boone and M. Wojciechowski for their help in administering the project. We are grateful to all of the families at the participating Simons Simplex Collection (SSC) sites, as well as the principal investigators (A. Beaudet, R. Bernier, J. Constantino, E. Cook, E. Fombonne, D. Geschwind, R. Goin-Kochel, E. Hanson, D. Grice, A. Klin, D. Ledbetter, C. Lord, C. Martin, D. Martin, R. Maxim, J. Miles, O. Ousley, K. Pelphrey, B. Peterson, J. Piggot, C. Saulnier, M. State, W. Stone, J. Sutcliffe, C. Walsh, Z. Warren, E. Wijsman). We appreciate obtaining access to phenotypic data on SFARI Base. Particular gratitude is owed Bernie Devlin for his input on statistical power calculations. J. Murdoch is also particularly grateful to his Ph.D. thesis committee, Drs. Kenneth Kidd and James Noonan, as well as Dr. State, whose insight and guidance were invaluable to this project.
Conceived and designed the experiments: ARG SJS MTM JDM MWS. Performed the experiments: JDM ARG MFW SA GTO MJR NMD NV ZW CS LG SYC. Analyzed the data: JDM ARG SJS JK MFW TVF MTM GTO MJR NMD ZW CS AJW BMN MJD. Contributed reagents/materials/analysis tools: BMN MJD. Wrote the paper: JDM MWS.
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