Calsequestrin is among the most abundant proteins in muscle sarcoplasmic reticulum and displays a high capacity but a low affinity for Ca2+ binding. In mammals, calsequestrin is encoded by two genes, CASQ1 and CASQ2, which are expressed almost exclusively in skeletal and cardiac muscles, respectively. Phylogenetic analysis indicates that calsequestrin is an ancient gene in metazoans, and that the duplication of the ancestral calsequestrin gene took place after the emergence of the lancelet. CASQ2 gene variants associated with catecholaminergic polymorphic ventricular tachycardia (CPVT) in humans are positively correlated with a high degree of evolutionary conservation across all calsequestrin homologues. The mutations are distributed in diverse locations of the calsequestrin protein and impart functional diversity but remarkably manifest in a similar phenotype in humans.
The sarcoplasmic reticulum (SR) is a high specialized membrane network that supports mechanical muscle functions requiring large fluxes of Ca2+. Consequently, the SR controls excitation–contraction coupling1,2,3 without compromising Ca2+ requiring cellular processes that are normally associated with the endoplasmic reticulum4. There are two well defined structural and functional regions of the SR in cardiac muscle: the longitudinal SR that runs parallel to the myofibrils and the junctional SR that forms multiple membrane contacts with T-tubule membrane contact sites5,6,7. SR-T-tubules membrane contact sites play an important role in initiation of the excitation–contraction coupling7. The longitudinal SR is enriched with Ca2+-ATPase (SERCA) which is responsible for the rapid removal of Ca2+ from the cytoplasm to initiate muscle relaxation1,5,6. The junctional SR is the primary site of Ca2+ release via the Ryanodine Receptor (RyR)/Ca2+ channel which triggers muscle contraction. The SR luminal Ca2+ binding protein calsequestrin is a high capacity, low affinity Ca2+ binding protein that forms oligomeric structures that regulate RyR activity via interactions with RyR, triadin and junctin1,8,9,10,11,12,13,14. There are two isoforms of calsequestrin, which are encoded by two different genes: cardiac calsequestrin (CASQ2) and skeletal muscle calsequestrin (CASQ1)14,15. The crystal structure of calsequestrin indicates that the protein contains three thioredoxin-like domains reminiscent of ER luminal oxidoreductases16,17.
Catecholaminergic polymorphic ventricular tachycardia (CPVT) is an inherited disease characterized by ventricular arrhythmias leading to sudden death18,19. CPVT results from defects in intracellular Ca2+ handling by cardiomyocytes. Two major variants have been associated with the CPVT disorder. The autosomal dominant form is associated with mutations in the cardiac ryanodine receptor (RyR2) gene and accounts for ~ 50% cases, while a recessive form with mutations in the cardiac isoform of calsequestrin (CASQ2) accounts for 2–5% cases. Other mutations also found in the CALM1, CALM2, CALM3 (encodes calmodulin1, 2, 3 respectively), and TRDN (encodes triadin) gene account for < 2% of CPVT cases20,21,22,23,24. Thirteen mutations in the CASQ2 gene have been identified in CPVT patients, in sudden death syndrome25,26, and three of them are non-synonymous polymorphisms (cSNP)24,27. Several biochemical and cell biological studies of R33Q, L167H, and D307H calsequestrin mutants indicate that these mutations lead to impaired Ca2+ storage and Ca2+ release from the SR22,24,25,26,27,28,29,30,31,32,33,34,35,36,37,38,39,40,41. Recently new calsequestrin mutations have been identified including K180R, D351G, G332R, and P329S27,39,40,42,43,44,45,46.
In this study, we examined the evolutionary constraints of the CPVT related calsequestrin mutations, and included Casq1, Casq2 and pre-duplicate calsequestrin in the phylogenetic analysis. We showed that calsequestrin is an ancient protein in the metazoan, and that the duplication of the calsequestrin gene took place after the divergence of the lancelet but before divergence of Chondrichthyes. We noted that calsequestrin mutations, associated with CPVT, positively correlated with an increase in the degree of evolutionary conservation of the mutated sites. Furthermore, we carried out biochemical and biophysical analysis of seven CPVT related mutants (R33Q, L167H, D307H, K180R), and whole exome sequencing variants (D351G, G332R, P329S) selected based on their linked to the human CPVT phenotype and located within highly conserved thioredoxin-like domain. The mutations are distributed in diverse locations of the calsequestrin protein but remarkably manifest in a similar phenotype in humans.
Emergence and specialization of calsequestrin within animals
Phylogenetic analysis of the two calsequestrin genes (casq1 and casq2) was carried out with the aim of clarifying the distribution and conservation of each paralogue across animals, and thus deduce the timing of the gene duplication event and relate this information to calsequestrin mutants responsible for CPVT. Homology searching was undertaken in 23 metazoan genomes and three outgroup lineages to identify calsequestrin homologues. We identified unambiguous calsequestrin homologues in most of the vertebrate and invertebrate lineages (Supp. Table S1). Furthermore, we revealed that Ciona intestinalis, B. floridae, and all taxa within the invertebrates possess a single calsequestrin gene, including taxa as deeply branched as Trichoplax and Nematostella (Fig. 1). We did not identify a calsequestrin homologue in the sponge Amphimedon despite rigorous searches. This is potentially due to a database error, but more intriguingly may well represent a loss of calsequestrin in this lineage, since preliminary searches of other sponge genomes also failed to identify calsequestrin homologues. Although the relative branching order of the basal lineages within animals is still disputed, with Nematostella or sponges as the deepest branch, calsequestrin is clearly an ancient protein within the metazoan (Suppl. Figs. S1 and S2).
Each of these lineages, as well the invertebrates and hemichordates, possess only a single calsequestrin gene, leaving the timing of when casq1 vs casq2 arose as an outstanding question. Preliminary phylogeny provided moderate support for the non-vertebrate sequences emerging basal to clades of the casq1 and casq2, thus being pre-duplicated versions (Suppl. Figs. S1). Further analysis focused on vertebrate gene sequences and using the lancelet sequences as an outgroup (Suppl. Fig. S2). The analysis robustly showed that the calsequestrin gene duplication that gave rise to casq1 and casq2 occurred after the divergence of the lancelet lineage but before the divergence of the Chondrichthyes (i.e. cartilaginous fish). We were unable to identify any calsequestrin sequences in the insect lineage. This likely represents a bona fide loss in this line given the positive identification of a homologue in the spider Parasteatoda tepidariorum.
We believe the Chondrichthyes and Avian taxa lost casq1 independently. We identified casq1 paralogues in the Chondrichthyes despite robustly classifying casq2 being present and the duplication having taken place prior to this point (Suppl. Fig. S2). The same was observed for the avian taxa sampled, suggesting that casq1 was lost independently in these three lineages. In mammalian muscles the two calsequestrin isoforms exhibit tissue specific expression47,48,49. Casq2 is expressed in cardiac and slow-twitch skeletal muscle, whereas Casq1 is expressed in adult fast-twitched muscle47,48,49. Cartilaginous fish as well as avian animals have both fast-twitch and slow-twitch skeletal muscles even though they appear to lack casq1.
Conservation of CPVT associated Casq2 mutants throughout animal kingdom
Having the evolutionary distribution of casq1 and casq2 allowed us to assess the conservation of sites in Casq2 proteins where calsequestrin mutations in the human CASQ2, have been associated with CPVT (Fig. 2A,B)24,50,51. We selected the following seven Casq2 mutants for further analyses: R33Q, L167H, D307H, K180R, P329S, G332R, and D351G (Fig. 2A,B). Many mutations are scattered across the three thioredoxin-like domains of Casq2 (Fig. 2A), but remarkably they all lead to a similar clinical outcome24,50. L167H, and D351G are conserved in Casq1 and Casq2 paralogues found in vertebrates but are variable in the pre-duplicated non-bilaterian (Fig. 2A). In contrast, positions R33Q, K180R, D307H, P329S and G332R are fully conserved across all calsequestrin homologues including pre-duplication Casq (Suppl. Fig. S2).
Ca2+ binding to Casq2 mutants
With the conservation of the relevant amino acid positions in hand, we next carried out biochemical and biophysical analysis of the Casq2 mutants in order to gain insight into the contribution of these mutations to the development of CPVT. First, we used microscale thermophoresis (MST) to investigate Ca2+ binding to Casq2 mutants. Mutation of Casq2 residues R33Q, L167H, K180R and D351G had no significant effect on Ca2+ binding to calsequestrin (Fig. 3A–D) with Kd values ranging from 0.872 ± 0.283 mM for wild-type to 1.052 ± 0.154 mM for the D351G mutant (Fig. 3H). However, P329S and G332R mutants exhibited altered Ca2+ binding affinities (Fig. 3E,F). Previous studies showed that R33Q, L167H, and D307H have highly reduced Ca2+ binding capacity17,31. Here, using label-free MST assay the D307H Casq2 mutant showed no measurable Ca2+ binding (Fig. 3G). Of the seven mutants associated with CPVT examined, only three exhibited altered Ca2+ binding properties.
Conformational changes and protein folding of Casq2 mutants
Casq2 undergoes conformational change upon Ca2+ binding, and this was monitored by circular dichroism (CD) analysis52. Upon adding Ca2+, wild-type Casq2 lost 18.3% α-helix and gained 16.79% β-sheet conformation (Fig. 4)52. CD spectra for K180R and D351G mutants overlapped with those of the wild-type Casq2 (Fig. 4C,D,E,F), indicating no effect of the K180R and D351G mutation on the protein conformation. However, the G332R and P329S mutants, showed altered sensitivity to Ca2+-induced conformational changes (Fig. 4E,F). This was in agreement with the reduced Ca2+ affinity of these mutants (Fig. 3). In contrast, the CD spectra of mutants R33Q, L167H, and D307H revealed increased α-helix content that was not sensitive to addition of Ca2+ (Fig. 4A,B,G; Table 1).
Next, we tested susceptibility of the Casq2 and Casq2 mutants to trypsin digestion to further analyze the impact of Casq2 mutations on protein folding. K180R and D351G mutants showed trypsin digestion patterns similar to wild-type protein indicating no major folding differences between these proteins (Fig. 5). In support of the CD analysis, R33Q, L167H, and D307H mutants showed limited trypsin susceptibility compared to wild-type protein both in the absence and presence of Ca2+ (Fig. 5). R33Q, L167H, and D307H mutants showed more α-helix (Fig. 4) and an increased sensitivity to trypsin digestion in the absent of Ca2+ (Fig. 5), indicative of altered protein folding. In agreement with Ca2+ binding (Fig. 3E,F) and CD analysis (Fig. 4E,F) trypsin digestion of P329S and G332R mutants also showed increased kinetics of digestion in the presence of Ca2+ (Fig. 5C,D), indicative of Ca2+-induced conformational changes of these mutants.
In agreement with previous study31, we found D307H to be more susceptible to trypsin digestion at high Ca2+ concentration, and conformational changes of this mutant were less sensitive to increased Ca2+ concentration (Figs. 4 and 5). In absence of Ca2+, D307H was shown to have trypsin susceptibility and CD spectra similar to wild-type protein17,31. In the present study we found D307H protein was more sensitive to trypsin digestion (Fig. 5). This was further supported with altered CD spectra of the D307H mutant (Fig. 4; Table 1). The differences between the two studies is likely due to different buffer conditions used for CD analysis and trypsin digestion. As previously reported53, L167H and R33Q were more susceptible to trypsin digestion in absence Ca2+ or presence of Ca2+ indicating altered protein folding of the mutants. This was supported by CD analysis (Fig. 4) and thermal denaturation assays (Fig. 6; Table 2).
Next, we used the Tycho NT.6 system to carry out thermal denaturation analysis of wild-type Casq2 and Casq2 mutants in a label-free environment as another indicator of protein folding. The analysis is based on measurement of the protein’s intrinsic tryptophan fluorescence and records a protein’s unfolding profile in real-time. Casq2 has 5 tryptophan residues all located in the third thioredoxin-like domain16,17 and fully buried in the hydrophobic core. K180R and D351G mutants showed an unfolding profile (Fig. 6A) and inflection temperature (Ti, proportionally to protein melting temperature) values (Fig. 6F,G; Table 2) similar to wild-type Casq2. Ti values for R33Q (52.55 °C) and G332R (47.23 °C) mutants, although close to the wild-type Casq2 (49.89 °C), were statistically different (Fig. 6C,E). P329S, G332R and D307H mutants showed minimal (for P329S and G332R mutants) to no detectable (for D307H mutant) unfolding transition (Fig. 6; Table 2). These mutants also showed a significantly higher initial ratio (350 nm/330 nm at 35 °C), indicating that tryptophan residues in P329S, G332R and D307H mutants were exposed to solvent, and the polarity of the local tryptophan environment was unchanged upon denaturing at higher temperature. The L167H mutant had an intermediate unfolding profile and significantly increased Ti value (Fig. 6; Table 2), indicating partially exposed tryptophan. The L167H mutation resulted in a partial disruption of the third thioredoxin-like domain and/or destabilized another protein domain, whereas, D307H, P329S, and G332R exhibited a large disruption in the third thioredoxin-like domain (Fig. 6; Table 2).
Ca2+ dependent polymerization of Casq2 mutants
Casq2 undergoes monomer to oligomer transition and oligomerization54. Upon binding to Ca2+, Casq2 undergoes reversible polymerization, and this affects Casq2 assembly to the junctional SR, which could have direct impact on SR Ca2+ supply and RyR2 regulation54. We tested for a Ca2+-dependent oligomerization of Casq2 mutants using disuccinimidyl suberate (DSS) cross-linker (Fig. 7) and native gel electrophoresis techniques (Fig. 8). Addition of Ca2+ to wild-type Casq2 increased oligomerization of the protein (Fig. 7). A similar pattern of Ca2+-dependent oligomerization was seen for K180R, D351G and D307H mutants (Fig. 7). Surprisingly, the D307H mutant that did not bind Ca2+ (Fig. 3) but showed Ca2+-dependent oligomerization indistinguishable from the wild-type Casq2 (Fig. 7) suggesting a role of Ca2+ in function of this mutant. R33Q, L167H, P329S and G332R mutants had increased Ca2+-dependent oligomerization whereas R33Q mutant showed no dependence on Ca2+ for oligomerization (Fig. 7). Under conditions of native electrophoresis, wild-type Casq2 and Casq2 mutants exhibited spontaneous oligomerization (Fig. 8) with R33Q, L167H and G332R mutants having a greater proportion in oligomeric form as compared to wild-type protein (Fig. 8). This was particularly evident for the R33Q and L167H mutants which existed predominantly (> 80% and > 60%, respectively) in an oligomeric form (Fig. 8).
Casq2 binding to IRE1α, an ER/SR stress sensor
Casq2 binds to IRE1α, an ER/SR stress sensor and squelches IRE1α activity55. We used MST thermophoresis to test whether Casq2 mutations affected Casq2 interaction with the luminal domain of IRE1α. R33Q, L167H, D307H, P329S, G332R and D351G bound to the luminal domain of IRE1α with similar kinetics and affinities as seen for wild-type protein (Fig. 9). However, the K180R mutant showed increased binding affinity (Fig. 9) indicating a stronger interaction between the K180R Casq2 mutant and the IRE1α luminal domain. We concluded that all Casq2 mutants tested bound to the IRE1α stress sensor.
Our phylogenetic analysis of the calsequestrin genes (casq2, casq1, and pre-duplication casq) revealed that calsequestrin is an ancient protein within the metazoan, and duplication of the calsequestrin gene took place after the divergence of the lancelet but before divergence of Chondrichthyes. Duplication of the calsequestrin gene allowed for the differentiation of a muscle-specific form of the protein, namely cardiac calsequestrin (casq2) expressed in cardiomyocytes. In the heart Ca2+ release from the calsequestrin (Casq2) rich junctional SR is initiated by the Ca2+-induced Ca2+ release mechanism. In skeletal muscle, where Casq1 is expressed, Ca2+ release from the junctional SR is initiated by the depolarization-induced Ca2+ release mechanism. Notably in mammalian species Casq1 is almost exclusively expressed in skeletal muscle (Suppl. Fig. S3). However, Gallus gallus appears to have lost the Casq1 gene and Casq2 is highly expressed in both heart and skeletal muscle tissue (Suppl. Fig. S3). Other non-mammalian vertebrates also did not show the tissue-specific expression patterns of Casq1 vs 2 observed consistently in mammalian species suggesting that this is a later evolved mammalian-specific trait.
We also discovered that the Chondrichthye and Avian taxa lost casq1 but retained the casq2. Arthropoda do not have the calsequestrin gene, although they have transversely striated muscle similar to the vertebrate skeletal muscle56 with well-developed transverse tubules associated SR cisternae57,58. Considering that Arthropoda move by means of their segmental appendages, they may not require high capacity Ca2+ stores.
Comparison between the evolutionary distribution of calsequestrin and the RyR proteins58 provides insight into the evolution of the excitation–contraction coupling system in metazoan muscles. While we were unable to identify calsequestrin homologues, RyR homologues have been found in the genomes of holozoans such as Capsaspora and choanoflagellates, suggesting that the RyR protein evolved first. The pairing of the calsequestrin and ryanodine receptors seems not to have been established as essential in non-vertebrate animals, given the lack of calsequestrin in sponges but presence in cniderians and ctenophores and the opposite for the RyRs58. The presence of the preduplicated RyR but absence of calsequestrin in insects suggests lack of essentiality of the paired regulation as well. However, both systems have been subject to expansions likely associated with two whole-genome duplication events near evolution of vertebrates58. Lineage-specific losses of the families are seen here as well in both cases. For example, amphibians lack the gene encoding RyR2, yet they express both forms of calsequestrin. These results support the notion of the appearance of multiple homologues of junctional SR proteins, including calsequestrin and RyR, which are associated with depolarization-induced Ca2+ release or Ca2+-induced Ca2+ release mechanisms58.
Phylogenetic analysis of casq2 within the metazoan revealed a high level of conservation, especially in the beta-sheet in the hydrophobic core of the third thioredoxin-like fold. The C-terminal Asp rich domain of Casq2, responsible for high capacity low affinity Ca2+ binding, remained highly conserved throughout many different species. Of note, the pre-duplicated calsequestrin C-terminal domain, however, contains limited numbers of acidic residues, indicating a relatively low Ca2+ binding capacity in this basal lineage59. There are many highly conserved amino acid residues distributed throughout Casq2 that may be under evolutionary constraints, and mutations in these regions of the protein are expected to impact protein structure and function60,61. Not surprisingly, Casq2 mutations associated with CPVT are dispersed throughout different protein regions, but all are highly conserved throughout metazoans some (R33Q, K180R, D307H, P329S and G332R) even including pre-duplication Casq. Because of a specific disease phenotype of Casq2 mutants, one a priori prediction is that the mutations associated with CPVT would be in sites conserved in Casq2 but divergent in Casq1 and preduplicates, providing gain-of function amino acid changes in Casq2 which were then disrupted by the disease phenotype-associated mutations. However, this was not what we observed. Instead we found strong conservation at these positions between the paralogues or indeed across all calsequestrin homologues. This suggests that the residues at these positions are critical for calsequestrin function. Specificity of cardiac disease seen with Casq2 mutants is likely due to the tissue-specific expression patterns of the paralogues. In humans there is little or no Casq1 paralogue expressed in cardiac tissue to compensate for Casq2 malfunction in CPVT.
For our biochemical studies, we have selected mutants linked to the human CPVT phenotype and located within highly conserved positions, namely, R33Q, L167H, K180R, D307H and three CASQ2 variants from whole-exome sequencing clinical testing, P329S, G332R, and D351G24,25,26,27,39,46,62,63. In agreement with previous reports25,30,34,36,53,64, our studies showed that Casq2R33Q, Casq2L167H, and Casq2D307H differed in their biochemical properties. Casq2D307H was reported to have significantly reduced Ca2+ binding capacity17. In this study, in label-free MST Ca2+ binding assay the D307H mutant showed no measurable Ca2+ binding and altered protein tertiary structure. R33Q and L167H mutants retained Ca2+ binding capacity but had increased sensitivity to tryptic cleavage and lost Ca2+-dependent polymerization.
The Casq2R33Q and Casq2L167H mutants form large oligomers insensitive to Ca2+, indicating that they lost Ca2+ depend polymerization, and are not able to depolymerize in response to Ca2+ depletion, a critical function that affects the RyR2 channel gating response to depletion of Ca2+ during muscle contraction54. Amazingly, Casq2D307H substitution from aspartic acid to histidine, in the highly conserved hydrophobic core of third thioredoxin-like domain of Casq2, results in the loss of low affinity Ca2+ binding to Casq2. This is likely due to disruption of the third thioredoxin-like domain, a highly conserved region in Casq2. Surprisingly, Casq2D307H polymerized in a Ca2+-dependent manner, and, just like the wild-type Casq2, it exhibited Ca2+-dependent confirmation changes29,31. Nevertheless, the loss of low affinity and high capacity Ca2+ binding sites, due to severe Casq2D307H misfolding, results in reduced Ca2+ storage at the junctional SR, and impaired Casq2/Ca2+-dependent regulation of RyR2 activity51,65. Animal studies revealed that in Casq2 D307H /D307H knock-in mice there is a reduction in the abundance Casq2 D307H protein29,66. Others reported no effect of D307H mutation of protein stability in either animal model or in cultured cardiomyocytes31,33,51,65. Expression of Casq2 L167H mutant did not affect the level of the endogenous wild-type Casq234. However, in R33Q knock-in mice there was a significant reduction in the abundance of Casq2R33Q/R33Q protein30. This likely contributes to the CPVT phenotype.
K180R, P329S, G332R, and D351G mutants have not been previously studied with respect to their biochemical properties. K180R is a newly identified Casq2 mutant, and the first autosomal dominant mutant found of Casq227. Knollman’s group recently reported a CPVT-like phenotype in a K180R heterozygous knock-in mouse model46. Here we discovered that the Casq2K180R protein has indistinguishable biochemical properties from the wild-type Casq2, including Ca2+ binding affinity, secondary structure and conformation change in response to increased Ca2+ concentration, protein flexibility and conformation stability upon trypsin proteolysis, protein folding, and Ca2+ dependent polymerization. Recently, crystal structure studies of the Casq2K180R maps the mutation to the filament-forming interface67, and it was proposed that disrupted Casq2 polymer formation may be responsible for Casq2 mutant-associated CPVT. Casq2 binds directly to the luminal domain of ER stress sensor IRE1α at the junctional SR to prevent the activation of IRE1α55. Interestingly, of all mutants tested in this study, only Casq2K180R showed altered binding to the luminal domain of IRE1α. Whether this is associated with CPVT remains to be established.
Casq2D351G39,42, Casq2P329S39 and Casq2G332R39 are three novel Casq2 variants39,42 located in a highly conserved third thioredoxin-like domain. Casq2P329S and Casq2G332R have been identified as heterozygous carrier39. They are localized in the hydrophobic core of the highly conserved beta-sheet of the third thioredoxin-like domain and are highly conserved throughout the metazoan including Casq1 and pre-duplicate Casq. To our knowledge, there have been no reports on the biochemical and biophysical analysis of these mutants. Casq2D351G showed protein folding and function similar to wild-type protein, whereas Casq2P329S and Casq2G332R showed similar properties to Casq2D307H, including severe disruption in protein folding and impaired Ca2+ binding, indicative of an important structural and functional role for the highly conserved beta-sheet in the third thioredoxin-like domain of Casq2.
Overall, the three CPVT disease causing Casq2 mutants (R33Q, L167H, D307H) and two heterozygous variants (P329S and G332R) may lead to CPVT via different mechanisms. The third thioredoxin-like fold domain contains one highly conserved beta-sheet consist of four beta-strands, which are essential for correct folding and Ca2+ binding, mutations in this region including D307H, P329S, and G332R, and all result in severely misfolded protein with reduced or lost Ca2+ binding. R33Q, L167H and K180R are located at the Casq2 front-to-front and back-to-back polymerization interface, causing dysfunction in the protein’s Ca2+ depend polymerization/depolymerization that would affect filament formation, as proposed by Titus et al.67. This may be the unifying feature of Casq2 mutants association with CPVT67.
The genomes used in the comparative genomics and phylogenetics analyses are publicly available and include the following from NCBI: Homo sapiens, Canis lupus familiaris, Bos taurus, Oryctolagus cuniculus, Sus scrofa, Rattus norvegicus, Mus musculus, Xenopus tropicalis, Gallus gallus, Taeniopygia guttata, Crocodylus porosus, Latimeria chalumnae, Danio rerio, Callorhinchus milii, Leucoraja erinacea, Branchiostoma floridae, Ciona intestinalis, Helobdella robusta, Drosophila melanogaster, Apis mellifera, Manduca sexta, Daphnia pulex, Parhyale hawaiensis, Parasteatoda tepidariorum, Caenorhabditis elegans, Nematostella vectensis, Mnemiopsis leidyi, Trichoplax adhaerans, Amphimedon queenslandica, Monosiga brevicollis, Salpingoeca rosetta, Capsaspora owczarzaki. Ensembl: Helobdella robusta. Skatebase.org: Leucoraja erinacea. hymenopteragenome.org: Apis mellifera. wfleabase.org: Daphnia pulex.
Comparative genomics, phylogenetic and sequence alignments
Using H. sapiens CASQ1 and CASQ2 sequences as queries, BLASTp (Basic Local Alignment Search Tool protein) searches were performed on the genomes of 28 metazoan organisms (Supplementary Table S1). Reciprocal BLAST was performed to verify the homology of significant hits obtained via forward BLAST. Predictions regarding the homology of a sequence were based on both the E-value and identity score. Hits that displayed the lowest E-value and greatest identity score in both the forward and reciprocal BLAST were predicted as being homologous. In cases of multiple homologous hits, the hit with the greatest identity score was predicted as being potentially orthologous. When no significant hits could be obtained using a BLASTp search, tBLASTn was used to search inside of the genome scaffolds. Additionally, HMMer was also used to search for sequences without significant BLASTp hits. Any potential HMMer hits were then verified using reciprocal BLAST.
For phylogenetic analyses, we used both RAxML consensus trees using 100 bootstraps and MrBayes Bayesian analysis trees with 10 million iterations achieving an average standard deviation of splits frequencies value of less than 0.01. Default parameters on CIPRES for RAxML-HPC v0.8 and MrBayes v3.2.6 on XSEDE were used with the following change for the RAxML trees: an LG4X protein matrix was used with the PROTGAMMA protein substitution model. The clades generated by the RAxML consensus trees were considered significant with node values of at least 50. MrBayes tree clades were considered significant with node probability values of at least 0.8. RAxML consensus trees were generated using Consensus v3.695, while the graphical representation of the phylogenetic results was generated using Figtree v1.3.1. The calsequestrin sequences found using comparative genomics were aligned using MUSCLE v3.8.31 and visualized using MESQUITE v3.2.
A pET22b E. coli expression vector containing full-length recombinant canine casq2 cDNA with a C-terminus 6xHis tag were used as template to obtain Casq2 mutants. Platinum pfx DNA polymerase (Invitrogen, 11708) was used for site-directed mutagenesis PCR with primers (Supp. Table S2). Methylated non-mutated template plasmids were digested with DpnI, and the correct mutations were confirmed by DNA sequencing. Seven CPVT-related Casq2 mutants (R33Q, L167H, K180R, D307H, P329S, G332R, D351G) were generated.
cDNA encoding wild-type canine cardiac casq2 and casq2 mutants was cloned into pET22b expression vector. Proteins were expressed in E. coli BL21(DE3) and purified. Cells were grown in LB medium until the A600 reaches 0.6 at 37 °C, then induced with 1 mM IPTG at 37 °C for 3 h. Cells were crashed into a buffer containing 50 mM Tris–HCl, pH 8.0, 300 mM NaCl, and 10% glycerol, then purified by using a HisTrap HP purification column (GE lifesciences, 17524701) and AKTA pure chromatography system (GE lifesciences 29018224). Purification was performed using binding buffer containing 50 mM Tris–HCl, pH 8.0, 300 mM NaCl, and protein eluted with buffer containing 50 mM Tris–HCl, pH 8.0, 300 mM NaCl, and 250 mM imidazole. The 6xHis tagged ER luminal domain of IRE1α (IRE1-NLD) was expressed in COS-1 cells and purified by Ni-NTA agarose chromatography55. Protein concentration was determined using Bio-Rad DC protein assay (Bio-Rad, 5000111) as recommended by the manufacturer. Protein concentration was also determined by measuring A280 absorbance using Nanovue plus spectrophotometer (GE Healthcare).
CD spectra were recorded on a Jasco model J-810 spectropolarimeter. Far UV CD spectra were collected with 4.82 μM protein in buffer containing 10 mM NaH2PO4, pH 7.4, and 5 mM KCl, as NaCl interferes with CD analysis. CD scans were recorded using a quartz cell with a path length of 1 mm, response time of 2 s, scan speed of 10 nm/min, and band width of 1.0 nm. Ca2+-induced changes in CD spectra were monitored in the presence of 1 mM of EGTA and 6 mM of CaCl2. CD spectra analysis was carried out at 24 °C. The final spectra was an average of 5 measurements, after baseline subtraction. Analysis of the spectra was performed using K2D368. The following calculations were performed for analysis:
Mean residue ellipticity was calculated with formula:
where [θ] with unit of Deg cm2dmol−1, θobs is the observed ellipticity in degrees, \(l\) is the optical path-length in cm, \(c\) is the protein concentration in g/ml, MRW is the mean residue molecular mass calculated with formula:
where \(M\) is a molecular mass of polypeptide chain in Da, and \(N\) is the number of amino acid in the chain.
MST and thermal denaturation analyses
MST analyses were carried out using a Monolith NT.115 instrument (Nano Temper Technologies, Germany) or Monolith NT.LabelFree instrument (Nano Temper Technologies, Germany). The ER-luminal domain of IRE1α (IRE1-NLD) was labelled using the Monolith NT Protein Labeling Kit RED-NHS (Nano Temper Technologies, cat# MO-C030) following the manufacture’s protocol. All experiments were carried out at room temperature in standard capillaries with 20% LED power (fluorescence lamp intensity) and 40% MST power (IR-laser intensity). The assay buffer contained 50 mM HEPES, pH 7.4, 150 mM KCl, 500 μM CaCl2, 250 μM EGTA, 0.05% Tween-20, and 2.5% glycerol. CaCl2 and EGTA concentrations were adjusted to obtain the desired free Ca2+ concentration: no Ca2+ (500 μM EGTA, 500 μM CaCl2), 5 mM (500 µM EGTA, 5.5 mM CaCl2). Free Ca2+ concentration was calculated using the Ca2+-EGTA Calculator TS v1.3 web tool69.
Ca2+ binding to wild-type Casq2 or Casq2 mutants were carried out using a Monolith NT.LabelFree instrument in standard capillaries with 20% LED power and 60% MST power. The proteins were incubated for 10 min in a buffer containing 50 mM HEPES, pH 7.4, 150 mM KCl, 0.1% pluronic F-127, and 50 μM EGTA. An increasing concentration of CaCl2 (0.01–20 mM, in 50 mM HEPES, pH 7.4, 150 mM KCl) was used. All MST data was analyzed by Monolith Affinity Analysis v2.2.6 software.
Thermal denaturation analysis of wild-type Casq2 or Casq2 mutants was carried out using Tycho NT.6. This label-free system is based on measurement of a protein’s intrinsic tryptophan fluorescence and records a protein’s unfolding profile in real-time as temperature is increased from 35 to 95 °C. Ten µl of 0.25 mg/ml protein was used in buffer containing 50 mM HEPES, pH 7.4, 150 mM KCl, 500 μM CaCl2, 250 μM EGTA, 0.05% Tween-20, and 2.5% glycerol.
Native polyacrylamide gel electrophoresis
To determining the oligomerization state of Casq2 or Casq2 mutants in the presence of the same free Ca2+ concentration (167 µM), a discontinuous Tris–glycine polyacrylamide gel system consisting of a 5% stacking gel and a 10% separation gel was used under non-denaturing conditions. Proteins were diluted 3 × with non-denaturing loading dye (240 mM Tris–HCl, pH 6.8, 30% glycerol, and 0.03% bromophenol blue). Proteins were separated in a Mini-PROTEAN electrophoresis chamber (BioRad) in a running buffer containing 25 mM Tris, pH 8.8, and 192 mM glycine, at 100 V, for 2 h at 4 °C. The proteins were stained with Stains-all solution70, Coomassie-blue, or transferred to nitrocellulose membrane for immunoblotting analysis.
Cardiac calsequestrin (Casq2) and mutant proteins were subjected to proteolysis in a buffer containing 50 mM HEPES, pH 7.4, 150 mM KCl, 500 μM CaCl2, 250 μM EGTA, 0.05% Tween-20, and 2.5% glycerol. CaCl2 and EGTA concentrations were adjusted to the desired free Ca2+ concentration: no Ca2+ (250 μM EGTA, 250 μM CaCl2), 5 mM (250 µM EGTA, 5.25 mM CaCl2). Free Ca2+ concentration was calculated using the Ca-EGTA Calculator TS v1.3 web tool69. Proteins (150 μg of protein in 200 μl) were incubated in a reaction buffer with the desired free Ca2+ concentration for 20 min at 25 °C before addition of trypsin at the trypsin/protein ration of 1:50 (w/w), and samples were taken for SDS-PAGE analysis at 1, 2, 5, 10, 20, 30, 60, and 120 min. The samples were mixed with 4 × SDS-PAGE sample buffer (Bio-Rad) containing PMSF, and boiled at 100 °C for 2 min before SDS-PAGE. All experiments were repeated 3 times with protein from 2 separate purifications. The gels were stained with Coomassie Brilliant Blue R-250 (Bio-Rad).
The homobiofunctional protein cross linker disuccinimidyl suberate (DSS) (Thermo Scientific Pierce, cat#:21555) was dissolved in DMSO at a final concentration of 10 mM55. Protein concentration of wild-type and Casq2 mutant proteins was determined using Bio-Rad DC protein assay and the proteins were diluted to a final concentration of 10 µM in a reaction buffer containing 50 mM HEPES, pH 7.4, 150 mM NaCl, 250 μM EGTA, 500 μM CaCl2, and 0.05% Tween-20. Proteins were incubated with 20-fold molar excess of DSS for 1 h at 22.5 °C. The reaction was then quenched for 15 min with 100 mM Tris pH 7.4 followed by SDS-PAGE (10% acrylamide). Proteins were transferred to nitrocellulose membrane follow by immunoblotting with mouse anti-6xHis antibodies (ThermoFisher, MA1-21315) or anti-calsequestrin antibodies (abcam, 3516).
Statistical analysis was performed using GraphPad Prism version 7.0. The Student’s t-test was used to compare the mean of two independent groups, and one-way Anova was used to compare the mean of three or more independent groups, with a p-value determined to be significant if less than 0.05.
Rossi, A. E. & Dirksen, R. T. Sarcoplasmic reticulum: The dynamic calcium governor of muscle. Muscle Nerve. 33(6), 715–731. https://doi.org/10.1002/mus.20512 (2006) (Epub 2006/02/16).
Eisner, D. A., Caldwell, J. L., Kistamas, K. & Trafford, A. W. Calcium and excitation-contraction coupling in the heart. Circ. Res. 121(2), 181–195. https://doi.org/10.1161/CIRCRESAHA.117.310230 (2017).
Reddish, F. N., Miller, C. L., Gorkhali, R. & Yang, J. J. Calcium dynamics mediated by the endoplasmic/sarcoplasmic reticulum and related diseases. Int. J. Mol. Sci. 18(5), 1024. https://doi.org/10.3390/ijms18051024 (2017) (Epub 2017/05/11).
Michalak, M. & Opas, M. Endoplasmic and sarcoplasmic reticulum in the heart. Trends Cell Biol. 19(6), 253–259. https://doi.org/10.1016/j.tcb.2009.03.006 (2009) (Epub 2009/05/05).
Wray, S. & Burdyga, T. Sarcoplasmic reticulum function in smooth muscle. Physiol. Rev. 90(1), 113–178. https://doi.org/10.1152/physrev.00018.2008. (2010) (Epub 2010/01/21).
Bers, D. M. Cardiac sarcoplasmic reticulum calcium leak: Basis and roles in cardiac dysfunction. Annu. Rev. Physiol. 76, 107–127. https://doi.org/10.1146/annurev-physiol-020911-153308 (2014).
Michalak, M. & Agellon, L. B. Stress coping strategies in the heart: An integrated view. Front. Cardiovasc. Med. 5, 168. https://doi.org/10.3389/fcvm.2018.00168. (2018) (Epub 2018/12/07).
Barone, V., Randazzo, D., Del Re, V., Sorrentino, V. & Rossi, D. Organization of junctional sarcoplasmic reticulum proteins in skeletal muscle fibers. J. Muscle Res. Cell Motil. 36(6), 501–515. https://doi.org/10.1007/s10974-015-9421-5 (2015).
Chopra, N. & Knollmann, B. C. Triadin regulates cardiac muscle couplon structure and microdomain Ca(2+) signalling: A path towards ventricular arrhythmias. Cardiovasc. Res. 98(2), 187–191. https://doi.org/10.1093/cvr/cvt023. (2013) (Epub 2013/02/12).
Costello, B. et al. Characterization of the junctional face membrane from terminal cisternae of sarcoplasmic reticulum. J. Cell Biol. 103(3), 741–753 (1986) (Epub 1986/09/01).
Lee, J. M. et al. Negatively charged amino acids within the intraluminal loop of ryanodine receptor are involved in the interaction with triadin. J. Biol. Chem. 279(8), 6994–7000. https://doi.org/10.1074/jbc.M312446200 (2004) (Epub 2003/11/26).
Kobayashi, Y. M., Alseikhan, B. A. & Jones, L. R. Localization and characterization of the calsequestrin-binding domain of triadin. 1 Evidence for a charged beta-strand in mediating the protein-protein interaction. J. Biol. Chem. 275(23), 17639–17646. https://doi.org/10.1074/jbc.M002091200 (2000) (Epub 2000/04/05).
Gyorke, I., Hester, N., Jones, L. R. & Gyorke, S. The role of calsequestrin, triadin, and junctin in conferring cardiac ryanodine receptor responsiveness to luminal calcium. Biophys. J. 86(4), 2121–2128. https://doi.org/10.1016/S0006-3495(04)74271-X. (2004) (Epub 2004/03/26).
Knollmann, B. C. New roles of calsequestrin and triadin in cardiac muscle. J. Physiol. 587(Pt 13), 3081–3087. https://doi.org/10.1113/jphysiol.2009.172098. (2009) (Epub 2009/05/20).
Gyorke, S., Stevens, S. C. & Terentyev, D. Cardiac calsequestrin: Quest inside the SR. J. Physiol. 587(Pt 13), 3091–3094. https://doi.org/10.1113/jphysiol.2009.172049. (2009) (Epub 2009/07/02).
Wang, S. et al. Crystal structure of calsequestrin from rabbit skeletal muscle sarcoplasmic reticulum. Nat. Struct. Biol. 5(6), 476–483 (1998).
Kim, E. et al. Characterization of human cardiac calsequestrin and its deleterious mutants. J. Mol. Biol. 373(4), 1047–1057. https://doi.org/10.1016/j.jmb.2007.08.055. (2007) (Epub 2007/09/21).
Baltogiannis, G. G. et al. CPVT: Arrhythmogenesis, therapeutic management, and future perspectives. A brief review of the literature. Front. Cardiovasc. Med. 6, 92. https://doi.org/10.3389/fcvm.2019.00092. (2019) (Epub 2019/08/06).
Mohamed, U., Napolitano, C. & Priori, S. G. Molecular and electrophysiological bases of catecholaminergic polymorphic ventricular tachycardia. J. Cardiovasc. Electrophysiol. 18(7), 791–797. https://doi.org/10.1111/j.1540-8167.2007.00766.x. (2007) (Epub 2007/06/21).
Priori, S. G. et al. Clinical and molecular characterization of patients with catecholaminergic polymorphic ventricular tachycardia. Circulation 106(1), 69–74. https://doi.org/10.1161/01.cir.0000020013.73106.d8. (2002) (Epub 2002/07/03).
Postma, A. V. et al. Absence of calsequestrin 2 causes severe forms of catecholaminergic polymorphic ventricular tachycardia. Circ. Res. 91(8), e21–e26. https://doi.org/10.1161/01.res.0000038886.18992.6b. (2002) (Epub 2002/10/19).
Nyegaard, M. et al. Mutations in calmodulin cause ventricular tachycardia and sudden cardiac death. Am. J. Hum. Genet. 91(4), 703–712. https://doi.org/10.1016/j.ajhg.2012.08.015. (2012) (Epub 2012/10/09).
Roux-Buisson, N. et al. Absence of triadin, a protein of the calcium release complex, is responsible for cardiac arrhythmia with sudden death in human. Hum. Mol. Genet. 21(12), 2759–2767. https://doi.org/10.1093/hmg/dds104. (2012) (Epub 2012/03/17).
Faggioni, M., Kryshtal, D. O. & Knollmann, B. C. Calsequestrin mutations and catecholaminergic polymorphic ventricular tachycardia. Pediatr. Cardiol. 33(6), 959–967. https://doi.org/10.1007/s00246-012-0256-1. (2012) (Epub 2012/03/17).
Terentyev, D. et al. Abnormal interactions of calsequestrin with the ryanodine receptor calcium release channel complex linked to exercise-induced sudden cardiac death. Circ. Res. 98(9), 1151–1158. https://doi.org/10.1161/01.RES.0000220647.93982.08. (2006) (Epub 2006/04/08).
Terentyev, D. et al. Modulation of SR Ca release by luminal Ca and calsequestrin in cardiac myocytes: Effects of CASQ2 mutations linked to sudden cardiac death. Biophys. J. 95(4), 2037–2048. https://doi.org/10.1529/biophysj.107.128249. (2008) (Epub 2008/05/13).
Gray, B. et al. A novel heterozygous mutation in cardiac calsequestrin causes autosomal dominant catecholaminergic polymorphic ventricular tachycardia. Heart Rhythm. 13(8), 1652–1660. https://doi.org/10.1016/j.hrthm.2016.05.004. (2016) (Epub 2016/05/10).
Lahat, H. et al. Autosomal recessive catecholamine- or exercise-induced polymorphic ventricular tachycardia: Clinical features and assignment of the disease gene to chromosome 1p13-21. Circulation 103(23), 2822–2827 (2001) (Epub 2001/06/13).
Song, L. et al. Calsequestrin 2 (CASQ2) mutations increase expression of calreticulin and ryanodine receptors, causing catecholaminergic polymorphic ventricular tachycardia. J. Clin. Investig. 117(7), 1814–1823. https://doi.org/10.1172/JCI31080. (2007) (Epub 2007/07/04).
Rizzi, N. et al. Unexpected structural and functional consequences of the R33Q homozygous mutation in cardiac calsequestrin: A complex arrhythmogenic cascade in a knock in mouse model. Circ. Res. 103(3), 298–306. https://doi.org/10.1161/CIRCRESAHA.108.171660. (2008) (Epub 2008/06/28).
Kalyanasundaram, A., Bal, N. C., Franzini-Armstrong, C., Knollmann, B. C. & Periasamy, M. The calsequestrin mutation CASQ2D307H does not affect protein stability and targeting to the junctional sarcoplasmic reticulum but compromises its dynamic regulation of calcium buffering. J. Biol. Chem. 285(5), 3076–3083. https://doi.org/10.1074/jbc.M109.053892. (2010) (Epub 2009/11/19).
Novak, A. et al. Cardiomyocytes generated from CPVTD307H patients are arrhythmogenic in response to beta-adrenergic stimulation. J. Cell Mol. Med. 16(3), 468–482. https://doi.org/10.1111/j.1582-4934.2011.01476.x. (2012) (Epub 2011/11/05).
Dirksen, W. P. et al. A mutation in calsequestrin, CASQ2D307H, impairs Sarcoplasmic reticulum Ca2+ handling and causes complex ventricular arrhythmias in mice. Cardiovasc. Res. 75(1), 69–78. https://doi.org/10.1016/j.cardiores.2007.03.002. (2007) (Epub 2007/04/24).
di Barletta, M. R. et al. Clinical phenotype and functional characterization of CASQ2 mutations associated with catecholaminergic polymorphic ventricular tachycardia. Circulation 114(10), 1012–1019. https://doi.org/10.1161/CIRCULATIONAHA.106.623793. (2006) (Epub 2006/08/16).
Chopra, N. & Knollmann, B. C. Cardiac calsequestrin: The new kid on the block in arrhythmias. J. Cardiovasc. Electrophysiol. 20(10), 1179–1185. https://doi.org/10.1111/j.1540-8167.2009.01531.x. (2009) (Epub 2009/07/01).
Bal, N. C. et al. The catecholaminergic polymorphic ventricular tachycardia mutation R33Q disrupts the N-terminal structural motif that regulates reversible calsequestrin polymerization. J. Biol. Chem. 285(22), 17188–17196. https://doi.org/10.1074/jbc.M109.096354. (2010) (Epub 2010/04/01).
Cacheux, M. et al. Interplay between triadin and calsequestrin in the pathogenesis of CPVT in the mouse. Mol. Ther. https://doi.org/10.1016/j.ymthe.2019.09.012. (2019) (Epub 2019/10/15).
Josephs, K., Patel, K., Janson, C. M., Montagna, C. & McDonald, T. V. Compound heterozygous CASQ2 mutations and long-term course of catecholaminergic polymorphic ventricular tachycardia. Mol. Genet. Genomic Med. 5(6), 788–794. https://doi.org/10.1002/mgg3.323. (2017) (Epub 2017/11/28).
Landstrom, A. P. et al. Interpreting incidentally identified variants in genes associated with catecholaminergic polymorphic ventricular tachycardia in a large cohort of clinical whole-exome genetic test referrals. Circ. Arrhythm. Electrophysiol. 10(4), e004742. https://doi.org/10.1161/CIRCEP.116.004742. (2017) (Epub 2017/04/14).
Rajagopalan, A. & Pollanen, M. S. Sudden death during struggle in the setting of heterozygosity for a mutation in calsequesterin 2. Forensic Sci. Med. Pathol. 12(1), 86–89. https://doi.org/10.1007/s12024-015-9733-1. (2016) (Epub 2015/12/17).
Liu, B. et al. Ablation of HRC alleviates cardiac arrhythmia and improves abnormal Ca handling in CASQ2 knockout mice prone to CPVT. Cardiovasc. Res. 108(2), 299–311. https://doi.org/10.1093/cvr/cvv222. (2015) (Epub 2015/09/28).
Neubauer, J. et al. Post-mortem whole-exome analysis in a large sudden infant death syndrome cohort with a focus on cardiovascular and metabolic genetic diseases. Eur. J. Hum. Genet. 25(4), 404–409. https://doi.org/10.1038/ejhg.2016.199. (2017) (Epub 2017/01/12).
Wong, C. H., Koo, S. H., She, G. Q., Chui, P. & Lee, E. J. Genetic variability of RyR2 and CASQ2 genes in an Asian population. Forensic Sci Int. 192(1–3), 53–55. https://doi.org/10.1016/j.forsciint.2009.07.019. (2009) (Epub 2009/08/28).
Liu, N., Ruan, Y. & Priori, S. G. Catecholaminergic polymorphic ventricular tachycardia. Prog. Cardiovasc. Dis. 51(1), 23–30. https://doi.org/10.1016/j.pcad.2007.10.005. (2008) (Epub 2008/07/19).
Laitinen, P. J., Swan, H. & Kontula, K. Molecular genetics of exercise-induced polymorphic ventricular tachycardia: Identification of three novel cardiac ryanodine receptor mutations and two common calsequestrin 2 amino-acid polymorphisms. Eur. J. Hum. Genet. 11(11), 888–891. https://doi.org/10.1038/sj.ejhg.5201061 (2003) (Epub 2003/10/23).
Wleklinski, M., Parikh, H. & Knollmann, B. C. An autosomal dominant mutation in calsequestrin 2 causes CPVT withotu changing protein levels. Biophys. J. 116, 95A-A96 (2019).
Damiani, E., Volpe, P. & Margreth, A. Coexpression of two isoforms of calsequestrin in rabbit slow-twitch muscle. J. Mus. Res. Cell Motil. 11, 522–530 (1990).
Fliegel, L., Leberer, E., Green, N. M. & MacLennan, D. H. The fast-twitch muscle calsequestrin isoform predominates in rabbit slow-twitch soleus muscle. FEBS Lett. 242(2), 297–300. https://doi.org/10.1016/0014-5793(89)80488-0. (1989) (Epub 1989/01/02).
Biral, D., Volpe, P., Damiani, E. & Margreth, A. Coexistence of two calsequestrin isoforms in rabbit slow-twitch skeletal muscle fibers. FEBS Lett. 299(2), 175–178. https://doi.org/10.1016/0014-5793(92)80241-8. (1992) (Epub 1992/03/09).
Eldar, M., Pras, E. & Lahat, H. A missense mutation in the CASQ2 gene is associated with autosomal-recessive catecholamine-induced polymorphic ventricular tachycardia. Trends Cardiovasc. Med. 13(4), 148–151. https://doi.org/10.1016/s1050-1738(03)00025-2. (2003) (Epub 2003/05/07).
Viatchenko-Karpinski, S. et al. Abnormal calcium signaling and sudden cardiac death associated with mutation of calsequestrin. Circ. Res. 94(4), 471–477. https://doi.org/10.1161/01.RES.0000115944.10681.EB. (2004) (Epub 2004/01/13).
Slupsky, J. R., Ohnishi, M., Carpenter, M. R. & Reithmeier, R. A. Characterization of cardiac calsequestrin. Biochemistry 26(20), 6539–6544. https://doi.org/10.1021/bi00394a038. (1987) (Epub 1987/10/06).
Valle, G. et al. Catecholaminergic polymorphic ventricular tachycardia-related mutations R33Q and L167H alter calcium sensitivity of human cardiac calsequestrin. Biochem. J. 413(2), 291–303. https://doi.org/10.1042/BJ20080163. (2008) (Epub 2008/04/11).
Manno, C. et al. Calsequestrin depolymerizes when calcium is depleted in the sarcoplasmic reticulum of working muscle. Proc. Natl. Acad. Sci. USA. 114(4), E638–E647. https://doi.org/10.1073/pnas.1620265114. (2017) (Epub 2017/01/11).
Wang, Q. et al. Two pools of IRE1alpha in cardiac and skeletal muscle cells. FASEB J. 33(8), 8892–8904. https://doi.org/10.1096/fj.201802626R. (2019) (Epub 2019/05/06).
Paniagua, R., Royuela, M., Garcia-Anchuelo, R. M. & Fraile, B. Ultrastructure of invertebrate muscle cell types. Histol. Histopathol. 11(1), 181–201 (1996) (Epub 1996/01/01).
Smith, D. S., Gupta, B. L. & Smith, U. The organization and myofilament array of insect visceral muscles. J. Cell Sci. 1(1), 49–57 (1966) (Epub 1966/03/01).
Mackrill, J. J. & Shiels, H. A. Evolution of excitation-contraction coupling. Adv. Exp. Med. Biol. 1131, 281–320. https://doi.org/10.1007/978-3-030-12457-1_12. (2020) (Epub 2019/10/28).
Bal, N. C. et al. The C-terminal calcium-sensitive disordered motifs regulate isoform-specific polymerization characteristics of calsequestrin. Biopolymers 103(1), 15–22. https://doi.org/10.1002/bip.22534. (2015) (Epub 2014/08/06).
Miller, M. P. & Kumar, S. Understanding human disease mutations through the use of interspecific genetic variation. Hum. Mol. Genet. 10(21), 2319–2328. https://doi.org/10.1093/hmg/10.21.2319. (2001) (Epub 2001/11/02).
Guo, H. H., Choe, J. & Loeb, L. A. Protein tolerance to random amino acid change. Proc. Natl. Acad. Sci. USA. 101(25), 9205–9210. https://doi.org/10.1073/pnas.0403255101. (2004) (Epub 2004/06/16).
Kumar, S. & Patel, R. Neutral theory, disease mutations, and personal exomes. Mol. Biol. Evol. 35(6), 1297–1303. https://doi.org/10.1093/molbev/msy085. (2018) (Epub 2018/04/25).
Vitkup, D., Sander, C. & Church, G. M. The amino-acid mutational spectrum of human genetic disease. Genome Biol. 4(11), R72. https://doi.org/10.1186/gb-2003-4-11-r72. (2003) (Epub 2003/11/13).
Qin, J. et al. Luminal Ca2+ regulation of single cardiac ryanodine receptors: Insights provided by calsequestrin and its mutants. J. Gen. Physiol. 131(4), 325–334. https://doi.org/10.1085/jgp.200709907. (2008) (Epub 2008/03/19).
Houle, T. D., Ram, M. L. & Cala, S. E. Calsequestrin mutant D307H exhibits depressed binding to its protein targets and a depressed response to calcium. Cardiovasc. Res. 64(2), 227–233. https://doi.org/10.1016/j.cardiores.2004.09.009. (2004) (Epub 2004/10/16).
Katz, G. et al. The role of mutant protein level in autosomal recessive catecholamine dependent polymorphic ventricular tachycardia (CPVT2). Biochem. Pharmacol. 86(11), 1576–1583. https://doi.org/10.1016/j.bcp.2013.09.012. (2013) (Epub 2013/09/28).
Titus, E. W. et al. The crystal structure of a cardiac calsequestrin filament reveals an atomic mechanism of calsequestrin-associated catecholaminergic polymorphic ventricular tachycardia. bioRxiv. https://doi.org/10.1101/672303 (2019).
Louis-Jeune, C., Andrade-Navarro, M. A. & Perez-Iratxeta, C. Prediction of protein secondary structure from circular dichroism using theoretically derived spectra. Proteins. 80(2), 374–381. https://doi.org/10.1002/prot.23188. (2012) (Epub 2011/11/19).
Schoenmakers, T. J., Visser, G. J., Flik, G., & Theuvenet, A. P. CHELATOR: An improved method for computing metal ion concentrations in physiological solutions. Biotechniques. 12(6):870–4, 6–9. (1992) (Epub 1992/06/01).
Campbell, K. P., MacLennan, D. H. & Jorgensen, A. O. Staining of the Ca2+-binding proteins, calsequestrin, calmodulin, troponin C, and S-100, with the cationic carbocyanine dye “Stains-all”. J. Biol. Chem. 258, 11267–11273 (1983).
Ashkenazy, H. et al. ConSurf 2016: An improved methodology to estimate and visualize evolutionary conservation in macromolecules. Nucleic Acids Res. 44(W1), W344–W350. https://doi.org/10.1093/nar/gkw408. (2016) (Epub 2016/05/12).
We thank Drs. L. Chen and Z. Tian (Agricultural Life and Environment Sciences, University of Alberta) for help with CD analysis. NLD-His6-KDEL expression vector was a generous gift from Dr. R. Kaufman. This work was supported by the Canadian Institutes of Health Research grants MOP-15291, MOP-15415 and PS-153325 to M.M; MOP-15291, MOP-86750 and PS-153325 to L.B.A.; Natural Sciences and Engineering Research Council of Canada grants to J.B.D., M.M. and L.B.A., SynAD Program and a generous donation from the Kenneth and Sheelagh McCourt family. T.P. is supported by a Women and Children’s Health Research Institute studentship and by a studentship award from the Multiple Sclerosis Society of Canada.
The authors declare no competing interests.
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Wang, Q., Paskevicius, T., Filbert, A. et al. Phylogenetic and biochemical analysis of calsequestrin structure and association of its variants with cardiac disorders. Sci Rep 10, 18115 (2020). https://doi.org/10.1038/s41598-020-75097-3
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