Atrial fibrillation (AF), the most common arrhythmia, is a growing epidemic with substantial morbidity and economic burden. Mechanisms underlying vulnerability to AF remain poorly understood, which contributes to the current lack of highly effective therapies. Recognizing mechanistic subtypes of AF may guide an individualized approach to patient management. Here, we describe a family with a previously unreported syndrome characterized by early-onset AF (age <35 years), conduction disease and signs of a primary atrial myopathy. Phenotypic penetrance was complete in all mutation carriers, although complete disease expressivity appears to be age-dependent. We show that this syndrome is caused by a novel, heterozygous p.Glu11Lys mutation in the atrial-specific myosin light chain gene MYL4. In zebrafish, mutant MYL4 leads to disruption of sarcomeric structure, atrial enlargement and electrical abnormalities associated with human AF. These findings describe the cause of a rare subtype of AF due to a primary, atrial-specific sarcomeric defect.
Primary cardiac electrical disorders commonly have a genetic basis and cause arrhythmias in otherwise healthy, young individuals without warning. Arrhythmias affecting the ventricle may manifest as sudden cardiac death, while atrial arrhythmias most commonly cause palpitations or stroke1,2,3,4,5. Collectively, genetic-based or inherited arrhythmia syndromes have become known as ‘channelopathies,’ reflecting the findings that mutations in genes encoding cardiac ion channels or their chaperones are the predominant cause of these conditions to date5. Considerable overlap exists in ion channel genes responsible for causing arrhythmia syndromes, with genetic defects in potassium, sodium and gap junction channel genes recognized to cause episodic arrhythmias arising from either the ventricular or atrial cardiac chambers or both6. Typically, these channel defects alter the action potential properties or intercellular electrical communication, promoting arrhythmia vulnerability. Thus far, only a single non-ion channel gene has been identified as a cause of a primary atrial arrhythmia syndrome7. In 2008, Hodgson-Zingman et al.7 reported a genetic mutation in the atrial natriuretic peptide gene, NPPA, in a large family with atrial fibrillation (AF), and demonstrated the novel observation of the effects of this neuro-hormone on the action potential of atrial myocardium.
Herein, we describe a family with early-onset AF that remained gene-elusive for known genetic causes of familial AF. Using an a priori approach, we performed whole-exome sequencing in both affected and unaffected family members and identified a novel genetic variant in the atrial-specific myosin light chain gene, MYL4, uniquely shared only by the affected individuals. We created a zebrafish model expressing the putative mutation, and show that zebrafish harbouring the mutation exhibit a phenotype characteristic of an atrial-specific cardiomyopathy and electrical abnormalities consistent with human AF. Although genetic diseases of the cardiac sarcomere are known to lead to ventricular cardiomyopathy and associated arrhythmia8, a primary atrial-specific inherited myopathy presenting as an atrial arrhythmia has never previously been described.
The index case in our study (Fig. 1a, III.3) presented with palpitations at 26 years of age, and revealed a family history of AF. Electrocardiography (ECG) showed AF with slow ventricular rate response (Fig. 1b). During periods of sinus rhythm and before medical therapy, extremely low amplitude P-waves and prolonged atrial–ventricular conduction (first-degree AV block) were observed, consistent with impaired atrial conduction. The patient had frequent recurrences of AF despite medical therapy. An intra-cardiac electrophysiological study demonstrated large areas of electrical silence within the left atrium, and some regions of the left and right atria showed rapid electrical signals consistent with ongoing atrial arrhythmia. A catheter ablation was performed. Despite a successful procedural end point, the patient continued to experience paroxysmal AF.
Family history revealed two additional symptomatic relatives. The patient’s mother (Fig. 1a, II.2) had first presented with AF at the age of 32 years and had a permanent pacemaker placed at the age of 48 years for bradycardia in the setting of permanent AF. Echocardiography revealed an enlarged left atrial volume index (LAVI; 40 ml m−2; normal <28 ml m−2), a profoundly decreased left atrial function index (LAFI)9 and normal biventricular size and function (Table 1). A 25-year-old sister was then investigated for complaints of palpitations (Fig. 1a, III.2). Rhythm monitoring confirmed frequent episodes of AF. During sinus rhythm, consistent with the observations of her sister, electrocardiography demonstrated very low amplitude P-waves and first-degree AV block (Fig. 1c). In addition, 48-h ambulatory heart rate monitoring showed profound sinus bradycardia with sinus rates as low as 33 beats per minute (b.p.m.; Table 1). Echocardiography showed an enlarged left atrium (LAVI 38 ml m−2) and decreased LAFI. Arrhythmia screening was offered to asymptomatic relatives, including another sister, two maternal uncles and two first cousins. Interestingly, a 22-year-old sister (Fig. 1a, III.1) and a 50-year-old uncle (Fig. 1a, II.3) were found with permanent AF, and a 20-year-old cousin (Fig. 1a, III.5) had an electrocardiogram also exhibiting low amplitude P-waves and first-degree AV block as observed in the index case, but no AF to date (Table 1). Overall, the predominant clinical phenotype represented in the family consists of AF, conduction disease and reduced left atrial function as measured by LAFI. All mutation carriers showed clinical penetrance, although full disease expressivity appears to be age-dependent, as subject III.5 at the age of 20 years has not yet shown evidence of AF or decreased left atrial function. Clinical details of the family are shown in Table 1.
Following genetic testing of the family which confirmed the absence of mutations in genes known to cause familial AF (GJA5, KCNA5, KCNE2, KCNJ2, KCNQ1, KCNH2, NPPA and SCN5A), the possibility of a mutation in a novel gene was considered. Whole-exome sequencing was performed in parallel on five clinically affected individuals (subjects II.2, II.3, III.1, III.2 and III.3), two unaffected family members (II.1 and II.5) and 10 arrhythmia-free, healthy control subjects. Bioinformatic analysis was aimed to identify novel protein-altering genetic variants unique to the affected individuals and absent from unaffected family members, parallel controls and large public exome databases. Six novel protein-altering variants were identified to be uniquely shared among the five affected individuals, including three variants that are highly conserved among species (Supplementary Table 1). Of these variants, only one, MYL4 p.Glu11Lys (E11K), affected a gene highly expressed in cardiac tissue—specifically, in atrial myocardium (Supplementary Table 2). MYL4 encodes the atrial-specific myosin essential light chain (ELC), a key sarcomeric component10. The E11K mutation resides within the protein’s N-terminus, a region demonstrated to bind F-actin10,11. Additional comprehensive sequencing of the coding region of MYL4 from DNA of 100 unrelated individuals with AF and no other cardiac co-morbidities did not yield any rare variants in MYL4.
To test pathogenicity of this MYL4 mutation, we generated a transgenic zebrafish line expressing the corresponding mutation in the zebrafish ortholog cmlc1 under control of the atrial-specific myh6 promoter (E17K transgenic). While the zebrafish heart is two-chambered, heart rate, P-wave duration, and PR, QRS and QT intervals are similar to those of humans12,13. A separate transgenic line expressing wild-type (WT) cmlc1 served as a control (WT transgenic). Quantitative PCR showed no statistical difference in cmlc1 expression between E17K transgenics and WT transgenics at larval stages, with decreased expression in the E17K adult (Supplementary Fig. 1). In addition, we assayed the gene expression profile of 13 other genes specific to atrial myocardial function, including major subunits of the L-type calcium channel (LTCC; cacna1c and cacna1d), the cardiac ryanodine receptor (ryr2b) and sarcomeric proteins (tnnc1a, tnnc1b, myh6 and actn2b). No difference in gene expression was observed for the selected calcium-related genes. A modest but statistically significant increase in expression was shown for troponin C genes tnnc1a and tnnc1b in the E17K transgenic adult atrium versus WT transgenic (P=0.003 and P=0.001, respectively; Supplementary Fig. 1). Whether this upregulation in troponin C in the E17K mutant represents a compensatory secondary change is uncertain.
Electrocardiography was performed on control and experimental adult fish. E17K transgenics exhibited specific electrocardiographic abnormalities recognized as surrogate risks for human AF (Table 2)14,15. Abnormalities included irregular sino-atrial impulse generation and bradycardia, and prolonged P-wave duration, reflecting slowed atrial conduction (Fig. 2a,b). Eight of 11 (73%) of E17K transgenics exhibited severe bradycardia (in fish, HR<80 b.p.m.) compared with 0 of 10 controls. E17K transgenics exhibited a 25% decrease in heart rate compared with controls (P=0.004, Mann-Whitney U test).
We evaluated whether E17K transgenic fish exhibited atrial enlargement consistent with atrial myopathy. Hearts were dissected from freshly euthanized adult fish and atrial and ventricular surface areas were measured. No statistical difference in ventricular surface area was observed between control and experimental fish (1.3±0.3 mm2 versus 1.6±0.2 mm2). In contrast, atrial areas were increased 1.6-fold for experimental fish compared with controls (1.74 versus 1.03 mm2, P=0.007; Fig. 2c). Strikingly, E17K transgenic atrial size exceeded ventricular size (atrial:ventricular area ratio 1.41 versus 0.65 for controls, P=0.01).
We then investigated whether the observed heart rhythm and atrial enlargement in E17K transgenic fish were correlated with sarcomeric disruption in larval or adult fish, given Myl4’s presence in atrial sarcomeres. WT transgenic and E17K transgenic fish were crossed into the Tg(myl7:LifeAct-GFP)s974 transgenic line, which labels myocardial F-actin with GFP and allows live imaging of myofibril organization16. In WT transgenic atria, imaged at 5 days post fertilization (d.p.f.), normal myofibril organization was seen (Fig. 3a). Compared with controls, myofibrils in E17K transgenic atria appeared disorganized, and in some myofibrils F-actin corresponding to individual sarcomeres appeared stippled and blurred, indicating abnormal organization of H-zones and Z-disks (Fig. 3b). Electron microscopy on adult zebrafish hearts was also performed, using WT hearts as a control. In contrast to WT, E17K transgenic atria had largely absent Z-disks (Fig. 3c,d).
Finally, we evaluated whether zebrafish myocardial function was affected before adulthood. Heart rate, and atrial and ventricular fractional shortening were measured for E17K and WT transgenic larvae at 3, 5 and 10 d.p.f. (Supplementary Fig. 2). There were no statistically significant functional differences between groups, suggesting that myofibrillar disarray, as described above, precedes atrial dysfunction and arrhythmia.
Myl4 and other myosin ELCs from vertebrate striated muscle have an additional ∼40 N-terminal amino acids that is absent in smooth muscle isoforms11,12. Although the crystal structure for shorter ELCs has been solved11, the structure of the extended N-terminus, where our identified mutation resides, is unsolved. Chemical cross-linking and deletion mutagenesis studies of the extended N-terminus have identified a major actin-binding site involving the first 11 residues of Myl4 (refs 11, 17, 18). This highly charged N-terminus binds directly to a cluster of C-terminal acidic residues at positions 360–364 of F-actin19,20,21. The interaction between the Myl4 N-terminus and actin is considered to be electrostatic, since increasing the ionic strength abolishes or significantly reduces the amount of crosslinking17,21,22.
A secondary structure model23 of the Myl4 N-terminus predicts a β-turn at residues 11–14, stabilized by hydrogen bond formation between residues E11 and K14 (Fig. 4a). Substitution of negatively charged glutamate (E11) for positively charged lysine (K11) predicts loss of the β-turn secondary structure (Fig. 4b). We next modelled the predicted quaternary structure and electrostatic interaction between E11–Myl4 and F-actin. An electrostatic interaction within a 5 Å distance is predicted to occur between negatively charged E11–Myl4 and K358 of actin—an interaction that is lost with the substitution of K11 in Myl4 (Fig. 5a,b). Thus, alterations in secondary structure and electrostatic interactions caused by E11K may impair direct binding of Myl4 to actin, thereby altering the sarcomere structure and function.
The phenotypes seen in human and zebrafish studies highlight the sarcomere as a centre for mechano-electrical integration. E17K transgenic zebrafish exhibited myofibrillar disarray, and electron microscopy showed absent Z-disks. Importantly, Z-disks couple electrical excitation to contraction with direct communication between the sarcolemma and the sarcomere via T-tubules formed through cell membrane invaginations24,25. T-tubules have a high density of LTCCs, and immunofluorescence confirms localization of LTCCs directly to Z-disks25,26. As the major mediator of calcium influx during phase 2 of the cardiac action potential, LTCC activation triggers ryanodine receptor activation leading to further release of calcium from the sarcoplasmic reticulum, and subsequent sarcomere activation and contractility26,27. Finally, F-actin is a core component of Z-disks. F-actin crosslinks adjacent sarcomeres via binding with α-actinin, allowing for uniform transmission of force across sarcomeres. Taken together, our findings suggest that the identified E11K-MYL4 mutation leads to destabilization of the F-actin–Z-disk complex, which may impair calcium signalling and cause atrial myopathy, leading to atrial arrhythmias. Given our findings, it is possible that more cases of early-onset AF may have features of subclinical atrial myopathy than previously recognized.
This study describes a previously unreported autosomal dominant form of heritable AF, with early age of onset, associated conduction system disease and atrial myopathy. It is compelling that a recent study describing large-scale whole-genome sequencing of the Icelandic population has identified a founder frameshift mutation in MYL4 present in 1.5% of the Southern Icelandic population that is associated with AF as a homozygous genotype28. Although we cannot exclude a potential contributing role to phenotype of the five other identified novel variants shared among affected individuals, their effect on an atrial-specific phenotype would be expected to be minimal at most, in light of their highest gene expression in tissues outside of the heart and absence of any currently known role in myocardial electrical or contractile function (Gene Ontology, Supplementary Table 2). Altogether, these findings and the modelling of E11K-MYL4 in zebrafish strongly support a causal relationship of MYL4 mutations for a unique subtype of human AF.
All patients provided written informed consent for genetic analysis and clinical records review under an approved research protocol from the University of Ottawa Heart Institute Research Ethics Board. ECG measurements, left ventricular ejection fraction and LAVI using biplane method of discs were performed according to the accepted clinical guidelines. LAFI was measured as described29.
DNA was prepared from venous blood or saliva samples from the index case and kindred members. Exome sequencing of five clinically affected and two unaffected kindred members, as well as 10 unaffected, unrelated controls was performed on the Agilent SureSelect 51 Mb exome capture kit, followed by 100-bp paired-end sequencing on the Illumina HiSeq 2000 platform to achieve high coverage. Sequencing generated a mean coverage of 64-fold, with 79 and 87% of target sequences at >20 × and 10 ×, respectively. Sequences were aligned to Human Genome version 19 (NCBI 37) using the Burrows–Wheeler Aligner. Single-nucleotide variant and indel calls were assigned quality scores using Genome Analysis Toolkit version 2.2 and annotated for novelty (using dbSNP, 1000 Genomes Project and NHLBI exome databases). Bioinformatic analysis was aimed to identify rare (MAF<0.01%) or novel protein-altering genetic variants unique to the affected individuals and absent from unaffected family members, parallel controls and large public exome databases. Novel, protein-altering variants uniquely shared among the five clinically affected individuals were all confirmed through PCR amplification and Sanger’s DNA sequencing. Conservation scores of novel variants were assigned a maximum score of 1 using PhastCons29 to quantify conservation in reference to 33 mammalian taxa. Mutation Taster30 and Polyphen-2 (ref. 31) softwares were used to predict the effect of protein-altering variants on protein structure and function. Gene ontology and tissue expression for each variant was summarized using the Gene Ontology Consortium (www.geneontology.org) and GeneCards (www.genecards.org) databases, respectively.
Transgenic zebrafish creation
The zebrafish MYL4 orthologue, cmlc1, was used as a template to create the corresponding E11K mutation using site-directed mutagenesis. WT and mutant cmlc1-coding sequence was cloned into an I-SceI vector under the control of the atrial myosin heavy chain (myh6) promoter; the vector also contained mCherry under the control of a crystallin alpha A (cryaa) promoter. Transgenesis was performed in TL background as described32. Tg(myh6:cmlc1E17K,cryaa:mcherry)s977 (termed E17K transgenic) and Tg(myh6:cmlc1WT,cryaa:mcherry)s978 (termed WT transgenic) zebrafish were maintained under standard conditions.
Electrocardiograms were performed for 2 min on anaesthetized adult transgenic zebrafish as previously described33, except that the two electrodes were placed under the left pectoral fin and on the pericardium, respectively. An Iso-DAM8A amplifier (World Precision Instruments Inc., Sarasota, FL) and Power 1401 data-acquisition interface (Cambridge Electronic Design, Cambridge, England) were used to acquire data. Data were analysed using Spike2 software, version 5.19 (Cambridge Electronic Design) and LabChart 8 (ADInstruments, Sydney, Australia). Fish that exhibited an injury current (ST elevation) on ECG were considered to have poor placement of electrodes and were excluded from analysis. For each fish, 10 consecutive heartbeats where a clearly identifiable baseline was seen were used to determine the average RR interval, PR interval and P-wave duration. Ten WT transgenic and 11 E17K transgenic fish were studied. Heart rate variability was calculated from the standard deviation of RR intervals.
Zebrafish adult heart measurements
For atrial and ventricular area measurements, adult zebrafish hearts were recovered as previously described16. Atrial and ventricular surface areas were measured using Fiji software (www.fiji.sc/). Fifteen WT transgenic and eight E17K transgenic fish were analysed. An unpaired two-tailed t-test was used to determine statistical significance between groups. P values of≤0.05 were considered statistically significant.
Zebrafish heart larval imaging and functional measurements
For live larval zebrafish myofibril imaging, WT transgenic and E17K transgenic fish were crossed into the Tg(myl7:LifeAct-GFP)s974 background to allow for imaging of myofibril organization as previously described16. A total of seven WT transgenic and eight E17K transgenic zebrafish were imaged. All experimental results were analysed in a blinded fashion.
Zebrafish larvae have hatched and swim independently. Larval heart rate and fractional shortening was performed by mounting larvae ventral side up, in 30-mm glass-bottom petri dishes (MatTek, Ashland, MA) in 1.2% low-melt agarose (GeneMate). When agarose had set (∼10 min), mounted larvae were covered with egg water and placed in a 28 °C incubator immediately adjacent to the microscope for ∼30 min. Mounted larvae were then removed one at a time and imaged immediately on a Stemi SV11 dissecting microscope (Carl Zeiss, Thornwood, NY) outfitted with a CCD camera at 20 frames per second (Toshiba IK-C43H 19). Measurements were taken from the first 10 s of video. Videos were then analysed with Fiji software (www.fiji.sc/) and atrial and ventricular fractional shortening was calculated as described34. Ten fish were measured per group.
Zebrafish heart electron microscopy
For electron microscopy, E17K transgenic and WT adult zebrafish hearts were dissected and immediately fixed in 2% glutaraldehyde, 1% paraformaldehyde in 0.1 M sodium cacodylate buffer pH 7.4, post-fixed in 2% osmium tetroxide in the same buffer, en bloc stained with 2% aqueous uranyl acetate, dehydrated in acetone, infiltrated and embedded in LX-112 resin (Ladd Research Industries, Burlington, VT). Specimens were ultrathin sectioned on a Reichert Ultracut S ultramicrotome and counter stained with 0.8% lead citrate. Grids were examined on a JEOL JEM-1230 transmission electron microscope (JEOL USA, Inc., Peabody, MA) and photographed with the Gatan Ultrascan 1000 digital camera (Gatan Inc., Warrendale, PA). Evaluation of images was performed by a cardiac pathologist (P. Ursell, UCSF) blinded to the labelling of samples, nature of the experimental perturbation and the clinical phenotype of affected individuals.
Total RNA was extracted from zebrafish tissues using Trizol reagent (GibcoBRL), purified using the Zymo RNA Clean & Concentrator-5 kit (Zymo Research), treated with DNAse (Qiagen) and reverse transcribed, as previously described35, using SuperScript IV reverse transcriptase (ThermoFisher). Real-time PCR was performed using an ABI Prism 7900HT Fast Real-Time PCR System (Applied Biosystems) and SensiFAST SYBR Hi-ROX Kit (Bioline). qPCR was performed comparing the expression of cmlc1 in the E17K transgenic relative to the WT transgenic at 5 d.p.f. (3 technical replicates per biological replicate; 3 biological replicates, 40 larvae per biological replicate). qPCR was also performed comparing the select genes in atria dissected from adult WT transgenic and E17K transgenic fish (three technical replicates per biological replicate; two biological replicates with one atrium per biological replicate; the third biological replicate was a pool of three adult atria). In addition to cmlc1, a subset of other genes were selected based on their cardiac expression, documented cardiac phenotypes in zebrafish and/or reported association with human AF. Exon-spanning primers were chosen where possible; no-RT controls for each biological replicate further confirmed insignificant genomic DNA contamination. Fold expression was calculated using the delta–delta Ct method, using elongation factor I alpha (eef1a1|1) as a reference gene. Statistical significance for each gene was calculated using a two-tailed t-test.
Secondary structure of WT and mutant N-termini of Myl4 was modelled using the QUARK protein structure prediction algorithm23. To model the interaction of the N-terminal region of MYL4 with F-actin, we adopted the approach described by Aydt et al.36 Briefly, the modelling utilizes known crystal structures demonstrating the 3D structure of actin (PDB 1ATN) and the crystal structure representing the interaction of chick myosin heavy chain, ELC and regulatory light chain with actin (PDB 2MYS). These crystal structures provide information on 116,559 atomic coordinates36. Aydt et al.36 modelled the binding of the N-terminal region of chick ELC (MLE1) onto these crystal structures. In our model, we substituted the homologous (76% identity) N-terminal region of MYL4 for the N-terminal region of chick ELC (MLE1) studied by Aydt et al36. and used the SWISS-MODEL program and the same atomic coordinates to model the tertiary structure of the interaction of WT and mutant N-termini of MYL4 with F-actin37. Residues within actin and MYL4 with the potential to interact with E11 on MYL4 were determined by examining the area within 5 Å of E11. Residues with hydrophobic properties or side chains incapable of interacting with E11 were discarded as possibilities. This analysis resulted in a predicted electrostatic interaction of MYL4-E11 with K358 on actin. The effect on the Myl4-actin interaction caused by substituting the positively charged K11 for negatively charged E11 was also modelled in a similar fashion38.
Accession codes: The MYL4 mutation encoding p.Glu11Lys has been deposited in the NCBI ClinVar database under accession # SCV000264340.
How to cite this article: Orr, N. et al. A mutation in the atrial-specific myosin light chain gene (MYL4) causes familial atrial fibrillation. Nat. Commun. 7:11303 doi: 10.1038/ncomms11303 (2016).
Ball, J., Carrington, M. J., McMurray, J. J. & Stewart, S. Atrial fibrillation: profile and burden of an evolving epidemic in the 21st century. Int. J. Cardiol. 167, 1807–1824 (2013).
Patel, N. J. et al. Contemporary trends of hospitalization for atrial fibrillation in the United States, 2000 through 2010: implications for healthcare planning. Circulation 129, 2371–2379 (2014).
Sorgente, A., Tung, P., Wylie, J. & Josephson, M. E. Six year follow-up after catheter ablation of atrial fibrillation: a palliation more than a true cure. Am. J. Cardiol. 109, 1179–1186 (2012).
Verma, A. et al. Discerning the incidence of symptomatic and asymptomatic episodes of atrial fibrillation before and after catheter ablation (DISCERN AF): a prospective, multicenter study. JAMA Intern. Med. 173, 149–156 (2013).
Marsman, R. F., Tan, H. L. & Bezzina, C. R. Genetics of sudden cardiac death caused by ventricular arrhythmias. Nat. Rev. Cardiol. 11, 96–111 (2014).
Roberts, J. D. & Gollob, M. H. Impact of genetic discoveries on the classification of lone atrial fibrillation. J. Am. Coll. Cardiol. 55, 705–712 (2010).
Hodgson-Zingman, D. M. et al. Atrial natriuretic peptide frameshift mutation in familial atrial fibrillation. N. Engl. J. Med. 359, 158–165 (2008).
Lopes, L. R. & Elliott, P. M. A straightforward guide to the sarcomeric basis of cardiomyopathies. Heart 100, 1916–1923 (2014).
Thomas, L., Hoy, M., Byth, K. & Schiller, N. B. The left atrial function index: a rhythm independent marker of atrial function. Eur. J. Echocardiogr. 9, 356–362 (2008).
Hernandez, O. M., Jones, M., Guzman, G. & Szczesna-Cordary, D. Myosin essential light chain in health and disease. Am. J. Physiol. Heart Circ. Physiol. 292, H1643–H1654 (2007).
Kazmierczak, K. et al. The role of the N-terminus of the myosin essential light chain in cardiac muscle contraction. J. Mol. Biol. 387, 706–725 (2009).
Arnaout, R. et al. Zebrafish model for human long QT syndrome. Proc. Natl Acad. Sci. USA 104, 11316–11321 (2007).
Milan, D. J., Jones, I. L., Ellinor, P. T. & MacRae, C. A. In vivo recording of adult zebrafish electrocardiogram and assessment of drug-induced QT prolongation. Am. J. Physiol. Heart Circ. Physiol. 291, H269–H273 (2006).
Alt, E. & Lehmann, G. Stroke and atrial fibrillation in sick sinus syndrome. Heart 77, 495–497 (1997).
Magnani, J. W. et al. P wave duration and risk of longitudinal atrial fibrillation in persons ≥60 years old (from the Framingham Heart Study). Am. J. Cardiol. 107, 917–921 (2011).
Reischauer, S., Arnaout, R., Ramadass, R. & Stainier, D. Y. Actin binding GFP allows 4D in vivo imaging of myofilament dynamics in the zebrafish heart and the identification of Erbb2 signaling as a remodeling factor of myofibril architecture. Circ. Res. 115, 845–856 (2014).
Yamamoto, K. & Sekine, T. Interaction of alkali light chain 1 with actin: effect of ionic strength on the cross-linking of alkali light chain 1 with actin. J. Biochem. 94, 2075–2078 (1983).
Schaub, M. C., Hefti, M. A., Zuellig, R. A. & Morano, I. Modulation of contractility in human cardiac hypertrophy by myosin essential light chain isoforms. Cardiovasc. Res. 37, 381–404 (1998).
Sutoh, K. Identification of myosin-binding sites on the actin sequence. Biochemistry 21, 3654–3661 (1982).
Milligan, R. A., Whittaker, M. & Safer, D. Molecular structure of F-actin and location of surface binding sites. Nature 348, 217–221 (1990).
Trayer, I. P., Trayer, H. R. & Levine, B. A. Evidence that the N-terminal region of A1-light chain of myosin interacts directly with the C-terminal region of actin. A proton magnetic resonance study. Eur. J. Biochem. 164, 259–266 (1987).
Timson, D. J., Trayer, H. R., Smith, K. J. & Trayer, I. P. Size and charge requirements for kinetic modulation and actin binding by alkali 1-type myosin essential light chains. J. Biol. Chem. 274, 18271–18277 (1999).
Xu, D. & Zhang, Y. Ab initio protein structure assembly using continuous structure fragments and optimized knowledge-based force field. Proteins 80, 1715–1735 (2012).
Pyle, W. G. & Solaro, R. J. At the crossroads of myocardial signaling: the role of Z-discs in intracellular signaling and cardiac function. Circ. Res. 94, 296–305 (2004).
Frank, D. & Frey, N. Cardiac Z-disc signaling network. J. Biol. Chem. 286, 9897–9904 (2011).
Kohl, T. & Lehnart, S. E. Imaging T-tubules: dynamic membrane structures for deep functions. Cardiovasc. Res. 98, 162–164 (2013).
Frisk, M. et al. Variable t-tubule organization and Ca2+ homeostasis across the atria. Am. J. Physiol. Heart Circ. Physiol. 307, H609–H620 (2014).
Gudbjartsson, D. F. et al. Large-scale whole-genome sequencing of the Icelandic population. Nat. Genet. 47, 435–444 (2015).
Schwarz, J. M., Cooper, D. N., Schuelke, M. & Seelow, D. MutationTaster2: mutation prediction for the deep-sequencing age. Nat. Methods 11, 361–362 (2014).
Adzhubei, I. A. et al. A method and server for predicting damaging missense mutations. Nat. Methods 7, 248–249 (2010).
Soroldoni, D., Hogan, B. M. & Oates, A. C. Simple and efficient transgenesis with Meganuclease constructs in zebrafish. Methods Mol. Biol. 546, 117–130 (2009).
Milan, D. J., Jones, I. L., Ellinor, P. T. & MacRae, C. A. In vivo recording of adult Zebrafish electrocardiogram and assessment of drug-induced QT prolongation. Am. J. Physiol. Heart Circ. Physiol. 291, H269–H273 (2006).
Arnaout, R., Reischauer, S. & Stainier, D. Y. Recovery of adult zebrafish hearts for high-throughput applications. J. Vis. Exp doi: 10.3791/52248 (2014).
Liu, J. et al. A dual role for ErbB2 signaling in cardiac Trabeculation. Development 137, 3867–3875 (2010).
McCurley, A. T. & Callard, G. V. Characterization of housekeeping genes in zebrafish: male-female differences and effects of tissue type, developmental stage and chemical treatment. BMC Mol. Biol. 9, 102 (2008).
Aydt, E. M., Wolff, G. & Morano, I. Molecular modeling of the myosin-S1(A1) isoform. J. Struct. Biol. 159, 158–163 (2007).
Biasini, M. et al. SWISS-MODEL: modelling protein tertiary and quaternary structure using evolutionary information. Nucleic Acids Res. 42, W252–W258 (2014).
Seeliger, D. & de Groot, B. L. Ligand docking and binding site analysis with PYMOL and Autodock/Vina. J. Comput. Aided Mol. Des. 24, 417–422 (2010).
We thank the patients and their families for their participation. We thank P. Ursell (University of California, San Francisco) for blinded evaluation of electron microscopy. This work was supported by grants NIH (F32HL110489) to S.R.C., NIH (HL54737) to D.Y.R.S., the Sarnoff Cardiovascular Research Foundation, NIH (K08HL125945-01) and American Heart Association (15GPSPG238300004) to R.A., the Deutsche Forschungsgemeinschaft (RE 3148/1-1) and the American Heart Association to S.R., Canadian Institutes of Health Research (MOP130263), the Heart and Stroke Foundation of Ontario (MC7449) and the Peter Munk Cardiovascular Molecular Medicine Research Chair (Toronto General Hospital) to M.H.G.
The authors declare no competing financial interests.
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Orr, N., Arnaout, R., Gula, L. et al. A mutation in the atrial-specific myosin light chain gene (MYL4) causes familial atrial fibrillation. Nat Commun 7, 11303 (2016). https://doi.org/10.1038/ncomms11303
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