- Short report
- Open Access
The Brugada syndrome mutation A39V does not affect surface expression of neuronal rat Cav1.2 channels
© Simms and Zamponi; licensee BioMed Central Ltd. 2012
- Received: 10 January 2012
- Accepted: 2 March 2012
- Published: 2 March 2012
A loss of function of the L-type calcium channel, Cav1.2, results in a cardiac specific disease known as Brugada syndrome. Although many Brugada syndrome channelopathies reduce channel function, one point mutation in the N-terminus of Cav1.2 (A39V) has been shown to elicit disease a phenotype because of a loss of surface trafficking of the channel. This lack of cell membrane expression could not be rescued by the trafficking chaperone Cavβ.
We report that despite the striking loss of trafficking described previously in the cardiac Cav1.2 channel, the A39V mutation while in the background of the brain isoform traffics and functions normally. We detected no differences in biophysical properties between wild type Cav1.2 and A39V-Cav1.2 in the presence of either a cardiac (Cavβ2b), or a neuronal beta subunit (Cavβ1b). In addition, the A39V-Cav1.2 mutant showed a normal Cavβ2b mediated increase in surface expression in tsA-201 cells.
The Brugada syndrome mutation A39V when introduced into rat brain Cav1.2 does not trigger the loss-of-trafficking phenotype seen in a previous study on the human heart isoform of the channel.
- L-type calcium channel
- Beta subunit
Cav1.2 is an L-type voltage-gated calcium channel that is indispensible for proper function of organs including the brain and the heart . Structurally, Cav1.2 channel complexes are composed of a pore-forming Cavα1 subunit, an accessory Cavα2δ subunit, and a Cavβ trafficking chaperone  which interacts with the Cavα1 subunit at the intracellular region linking the first two transmembrane domains [3–5]. Extensive alternate splicing of Cav1.2 between neuronal and cardiac backgrounds alters channel structure and function, as does the type of Cavβ subunit that is expressed in a given tissue [6–9]. Gain of function mutations in Cav1.2 channels may result in a multi-organ disease known as Timothy syndrome which is characterized by cardiac symptoms such as a prolonged Q-T interval, arrhythmias and sudden cardiac death (SCD); as well as immune dysfunction and autism . A loss of Cav1.2 function on the other hand, can give rise to a heart specific disorder termed Brugada syndrome whose phenotype consists of a shortened Q-T interval, ventricular fibrillation and SCD . Brugada syndrome has been associated with a gain of function in KCNE potassium channels , as well as a loss of function of Nav1.5 (15% of all cases) and Cav1.2/Cavβ (5% of all cases) [1, 12]. How exactly increased Cav1.2 activity yields a disease phenotype in heart and brain, whereas reduced function selectively affects the heart is unknown, but may be explained by tissue-specific splice isoforms of the channel. Recent reports of splice isoform specific effects of mutations in P/Q-type and T-type calcium channels [13, 14] may suggest that the tissue selective effect of Brugada syndrome mutations could be related to Cav1.2 channel sequences that are specific to the heart.
Recently a point mutation in the N-terminus of Cav1.2 (A39V) was identified in a patient with Brugada syndrome. This mutation resulted in a striking loss-of-function by way of disabled surface trafficking of the L-type channel complex . The defective surface expression of A39V-Cav1.2 persisted upon coexpression of the cardiac Cavβ2b subunit, indicating that the effects of the mutation dominated over the well documented protective effect of Cavβ. This may be due to the possibility that intracellular linkers other than the I-II linker modulate surface expression of Cav1.2. Alternate splicing in the amino terminus of the channel can alter cell surface trafficking [6, 15, 16]. In addition an N-terminal splice variant specific to the heart termed the 'long variant', imparts PKC regulation upon the channel, while another shorter variant found in both heart and brain does not [17, 18]. What is more important is that this second N-terminal variant is common to both the brain isoform used in our study and the cardiac channel used to test A39V-Cav1.2 previously. Other key sequence differences between cardiac and neuronal Cav1.2 variants do exist however, as do differences between human and rat channels, which are approximately 95% homologous (see Additional file 1: Figure S1).
The fact remains that the patient carrying A39V-Cav1.2 did not present with neurological symptoms raising the possibility that this mutation does not affect the sub-cellular trafficking of neuronal Cav1.2 channels.
To test this hypothesis we introduced the A39V mutation into rat brain Cav1.2 channels and examined its functional consequences in tsA-201 cells. Unlike in previous work with cardiac Cav1.2, we show that neuronal A39V-Cav1.2 retains Cavβ2b-dependent increases in surface expression, as well as total expression. We did not detect any biophysical differences between A39V-Cav1.2 and WT-Cav1.2 in the presence of either a cardiac or neuronal Cavβ subunit. We thus conclude that splice isoform differences between cardiac and neuronal Cav1.2 channels underlie the absence of a brain phenotype for the A39V Brugada mutation.
Wild type (WT) rat calcium channel subunit cDNAs encoding Cav1.2 (α1C), Cavβ1b and Cavα2δ1 subunits, as well as the pMT2 vector were generously donated by Dr. Terry Snutch (University of British Columbia, Vancouver, BC). Rat Cav1.2 has a polymorphism (glycine at amino acid position 57) adjacent to the A39V Brugada mutation locus which is not present in the human cardiac isoform. To facilitate comparison with previous work , we mutated rat Cav1.2 at position 57 to aspartic acid using QuickChange Site-Directed Mutagenesis Kit (Stratagene) as per manufacturer's instructions. The primer used for the G57D Cav1.2 mutagenesis was GGCAGGCAGCCATCGACGCCGCCCGGCAGGCC and its molecular complement. The A39V mutation was then constructed in both non-tagged and HA tagged Cav1.2 constructs using the primer AATGCAGCTGCAGGACTTGTCCCCGAGCACATCCCTACTCC. Following mutagenesis and cDNA preparation all clones were sequenced to verify the presence of desired mutations and overall sequence fidelity. The HA tagged version of Cav1.2 used has been previously described . The Cavβ2b construct was generously donated by Dr. Henry Colecraft (Columbia University, New York, USA). GenBank™ accession numbers for the clones used are as follows: Cav1.2 [M67515], Cavβ1b [NM017346], Cavβ2b [AF423193.1], and Cavα2δ1 [AF286488].
Tissue culture and transient transfection
Human embryonic kidney tsA-201 cells were grown and transiently transfected using the calcium phosphate method as described previously . Transfection solutions for individual culture dishes contained a mixture of cDNA expression vectors, with the following quantities of cDNA expression constructs used: WT, or A39V calcium channel Cav1.2 subunit (3 μg), Cavβ subunit (3 μg), Cavα2δ1 (3 μg) and in addition for electrophysiology transfections, 0.25 μg pEGFP marker vector (Clontech). Non-tagged Cav1.2 clones were used for electrophysiology, while HA-tagged clones were transfected for all other experiments. Transfections which lacked a Cavβ subunit included 3 μg of pMT2 vector. Twelve hours post-transfection cells were washed once with PBS (pH 7.4), supplemented with fresh DMEM, and allowed to recover for 12 h. To prevent overgrowth for electrophysiology, cells were transferred to a 29°C incubator and maintained for 48-72 h prior to voltage-clamp recording. For immunoprecipitation/Western blot and immunofluorescence experiments cells were kept at 37°C for 48-72 h after PBS/DMEM treatment and grown to 75-85% confluence.
Immunoprecipitation and Western blotting
Cultured tsA-201 cells were transiently transfected as described above with HA tagged channels for immunoprecipitation assays and were lysed with a modified RIPA buffer (in mM; 50 Tris, 130 NaCl, 0.2% triton X-100, 0.2% NP-40, 5 EGTA, pH 7.4). Lysis was carried out on ice for 15 min after which cells were centrifuged at 13, 000 rpm for 5 min at 4°C. Supernatants were then transferred to new tubes and solubilized proteins were incubated with 50 μl of Protein G beads (Pierce/Promega) and 1 μg of HA antibody (Roche) overnight while tumbling at 4°C. Total inputs were taken from whole cell samples representing 2.5% of the total protein and probed for alpha-actin (Sigma). Immunoprecipitates were washed once with the previously described modified RIPA buffer and a second time with a high salt RIPA buffer (in mM 500 NaCl, 50 Tris, 0.1% triton X-100, 0.1% NP-40, pH 7.4) and a final time with PBS (pH 7.4). Following washing, beads were aspirated to dryness and Laemmli buffer was added to samples before incubating at 96°C for 10 min. Eluted samples were loaded on the appropriate percentage Tris-glycine gel and resolved using SDS-PAGE. Samples were transferred to 0.45 μm PDVF membranes (Millipore) and western blot analysis performed using 1/1000 anti-HA (Covance), or 1/1000 anti-actin (Sigma). GE Healthcare horseradish peroxidase-linked secondary antibodies of appropriate species (mouse and rabbit) were used at 1/10000 dilution. Image J (National Institute of Health) was used to quantify the integrated density of protein on Western blots. For each blot the background signal was subtracted from experimental integrated densities to obtain sample values. Background subtracted values for HA signal were then divided by background subtracted actin signal to obtain the HA/actin ratio.
Cultured tsA-201 cells were transiently transfected as described above with HA tagged channels. Seventy two hours after transfection cells were fixed with 4% paraformaldehyde, and immunostained with anti-HA (1/1000, Roche). Alexa Fluor 594-conjugated goat α-rat IgG antibody (Molecular Probes, 1/1000) was used as the secondary antibody. Cells were imaged using a Zeiss LSM-510 Meta confocal microscope with a 40 × 1.2NA water immersion lens in the inverted position. The AF-594 antibody was visualized by excitation with a HeNe laser (543 nm) and emission detected using a 585-615-nm band pass filter. Image acquisition was performed with identical gain, contrast, laser excitation, pinhole aperture (fully open), scan size and laser scanning speed for all samples. Quantification of fluorescent signal was done following offline threshold adjustment with Image J. To obtain values for fluorescence/cell the total fluorescence per image was divided by the number of cells above threshold in that image.
Cav1.2 voltage clamp recordings
Glass cover slips carrying cells expressing A39V or WT Cav1.2 channels (no HA tag) were transferred to a 3.5-cm culture dish (Corning) containing external recording solution consisting of 20 mM BaCl2, 1 mM MgCl2,10 mM HEPES, 10 mM Glucose and 136 mM CsCl (pH 7.4 adjusted with CsOH). Micro-electrode patch pipettes were pulled and polished using a DMZ- Universal Puller (Dagan Corporation) to a typical resistance of 3-5 MÙ. Internal pipette solution consisted of 110 mM CsCH3SO3, 20 mM TEA-Cl, 10 mM EGTA, 2 mM MgCl2 and 10 mM HEPES (pH 7.2 adjusted with CsOH).
Whole cell patch clamp recordings were performed in voltage-clamp mode using an Axopatch 200B amplifier (Axon Instruments) linked to a personal computer with pCLAMP software version 9.2. Series resistance was compensated by 85%, leak currents were negligible, and the data were filtered at 5 kHz. Individual pEGFP expressing cells were held at -100 mV. For steady state inactivation curves, we applied 4.5 s conditioning depolarizations, followed by a test pulse to +10 mV for 0.5 s. Individual sweeps were separated by 15 s. All stable cells with detectable inward current at 0 mV were used to calculate current density. Only those cells whose whole cell current voltage relationships could be fit with the modified Boltzmann equation, I = (1/(1 + exp(-(Va-V)/S)))*(V-Erev)*Gmax, where 'I' is current, 'Va' is half-activation potential, 'V' is membrane potential, 'Erev' is reversal potential, S is the slope factor, and 'Gmax' is slope conductance, were used for determination of voltage-dependent properties. As well, only cells whose steady-state inactivation could be fit by the Boltzmann equation, I/Imax = A2 + A1/(1 + exp((V-Vh)/S)), where 'I/Imax' is normalized current, 'A2' is the non-inactivating fraction, 'A1' is inactivating fraction, 'V' is membrane potential, S is the slope factor, and 'Vh' is half inactivation potential, were used to calculate voltage-dependent properties of steady-state inactivation.
All electrophysiological data were analyzed using Clampfit version 9.2 (Axon Instruments) and fit in Origin 7 (Origin Lab Corporation). Image J was used to quantify the integrated density units (IDUs) of protein on Western blots as describe above. For quantification of fluorescent images Image J was used as described above yielding units of Arbitrary Light Units (ALUs). Statistical analyses for both biochemical and electrophysiological data were carried out using Origin 7. All sample means are reported +/- SEM. Statistically significant differences between means were assessed using student's t-test, or one-way ANOVA at 95% confidence level as appropriate.
Brugada syndrome mutations contribute to cardiac disease by shortening the Q-T segment of contraction, leading to arrhythmia and sudden cardiac death . Functional changes that reduce Cav1.2 conductance can lead to Brugada syndrome, but so can mutations that reduce the number of channels in the cell membrane due to compromised cell surface trafficking. It was shown that a point mutation (A39V) in the N-terminus of a cardiac isoform of Cav1.2 severely limited membrane expression of the channel even upon coexpression of the ancillary Cavβ2b subunit . This is unexpected considering that the Cavβ subunit promotes ER export and surface trafficking of the channel by binding the intracellular linker connecting domains I and II of the calcium channel α1 subunit [16, 20]. Given that Brugada syndrome does not involve compromised brain function, we wondered if the A39V mutation might trigger a similar loss-of-trafficking phenotype in neuronal Cav1.2 channels.
The Cavβ subunit has been shown to increase total expression of Cav1.2 by binding to the I-II intracellular linker of the channel and preventing ER associated degradation (ERAD) . We therefore tested whether A39V-Cav1.2-HA total protein was increased upon coexpression of Cavβ2b and whether A39V-Cav1.2-HA expressed like WT-Cav1.2-HA without a Cavβ subunit (Figure 1C). Immunoprecipitation of the channels combined with semi-quantification against alpha-actin yield demonstrated that, in the absence of a Cavβ subunit, the integrated density of A39V-Cav1.2-HA (2.56 +/- 0.48 IDUs) was significantly less than WT-Cav1.2-HA (4.33 +/-0.66 IDUs, p = 0.04 by students t-test) (Figure 1D). Therefore, A39V-Cav1.2 is either produced to a lesser extent, or degraded more effectively than WT-Cav1.2. Since both Cav1.2 constructs were transfected identically and driven by the same constitutive promoter, the latter of these two possibilities appears more likely. Our data also reveal that coexpression of either Cavβ2b (5.20 +/-0.25 IDUs) (Figure 1C) or Cavβ1b (5.69 +/-0.62 IDUs) (Additional file 2: Figure S2B), results in a significant increase in A39V-Cav1.2-HA protein levels (p = < 0.05 by ANOVA) (Figure 1D). This confirms that the protective role of the Cavβ subunit is maintained in the A39V-Cav1.2 channel. Interestingly, total WT-Cav1.2-HA protein levels were increased upon coexpression of Cavβ1b (5.05 +/- 0.79 IDUs), but to a lesser degree than described by our lab previously for a Cav1.2. We attribute this to a different amino acid sequence in the N-terminus of the channel , perhaps suggesting that the N-terminus is involved in regulating Cav1.2 channel stability.
Current densities and voltage-dependent properties of A39V-Cav1.2 without Cavβ, with Cavβ2b, or with Cavβ1b
Current Density (pA/pF)
V1/2 Activation (mV)
Slope of Activation (mV)
V1/2 Steady State Inactivation (mV)
Slope of Steady State Inactivation (mV)
Cav1.2 + Cavα2δ
-4.4 +/- 0.5
-9.1 +/- 1.3
4.7 +/- 0.7
6.9 +/- 0.6#
A39V-Cav.2 + Cavα2δ
-3.3 +/- 0.5
-11.7 +/- 1.5
4.6 +/- 0.9
-7.3 +/- 1.9
11.8 +/- 1.4#
Cav1.2 + α2δ + Cavβ2b
-9.1 +/- 1.4 *
-3.8 +/- 0.8
10.2 +/- 1.4
-7.1 +/- 1.7
11.1 +/- 1.8
A39V-Cav1.2 + Cavα2δ + Cavβ2b
-9.5 +/- 1.3 **
-3.0 +/- 1.4
13.0 +/- 2.0
-5.2 +/- 2.8
11.5 +/- 1.2
Cav1.2 + Cavα2δ + Cavβ1b
-10.6 +/- 1.1 *
-9.0 +/- 0.8
8.8 +/- 1.2
-6.3 +/- 1.1
8.4 +/- 1.2
A39V-Cav1.2 + Cavα2δ + Cavβ1b
-8.3 +/- 1.0 **
-6.4 +/- 1.1
8.1 +/- 0.9
-6.8 +/- 1.6
9.3 +/- 0.8
It has been demonstrated that mutations in the cardiac Cavβ2b subunit can affect inactivation of Cav1.2 in order to produce a Brugada phenotype . Furthermore, the N-terminus of Cav1.2 has been shown to affect inactivation of the channel in a manner dependent on the Cavβ subunit . We therefore tested whether the steady-state inactivation properties of A39V-Cav1.2 were different from those of WT-Cav1.2 in the presence of a Cavβ subunit. In the presence of either Cavβ2b (Figure 2B), or Cavβ1b (Additional file 2: Figure S2D) the steady-state inactivation properties of A39V-Cav1.2 are not significantly different from WT-Cav1.2. However, in the absence of the Cavβ subunit, A39V-Cav1.2 displays a significant increase in the slope of the inactivation curve (11.8 +/- 1.4 mV) which is significant when compared to WT-Cav1.2 (6.9 +/- 0.6 mV, p = < 0.01 students t-test). Furthermore, the A39V-Cav1.2 channel underwent a greater extent of total inactivation compared to the WT channel as denoted by red asterisks in Figure 2B (test potentials of -20,-10, +10, and +30 mV, p = < 0.05 by students t-test). This behavior of A39V-Cav1.2 could in principle be interpreted as a loss-of-function; however, as this occurs only in the absence of Cavβ, this effect will not likely manifest itself in native cells.
Here, we examined the Cavβ-dependence of the Brugada mutation A39V with regard to surface trafficking, total expression and function within the neuronal Cav1.2 isoform. Contrary to previous work on the cardiac isoform of Cav1.2 showing a loss of cell surface trafficking of A39V-Cav1.2 in the presence of Cavβ2b, we find that both cardiac Cavβ2b and neuronal Cavβ1b equally regulate the neuronal forms of mutant and WT Cav1.2 channels, and that the mutation does not alter the behavior of the neuronal channel in the absence of the Cavβ subunit. The concept of channel isoform-dependent effects of disease causing mutations is not without precedent [13, 14] and in the case of the Brugada mutation A39V may perhaps explain why patients afflicted with this mutation do not exhibit a neuronal phenotype.
Work from our laboratory is supported by the Canadian Institutes of Health research, the Natural Sciences and Engineering Research Council, and the Heart of Stroke Foundation of Alberta and the Northwest Territories. BAS is supported by a studentship from Alberta Innovates-Health Solutions (AI-HS). GWZ is an AI-HS Scientist and a Canada Research Chair.
- Antzelevitch C, et al: Loss-of-function mutations in the cardiac calcium channel underlie a new clinical entity characterized by ST-segment elevation, short QT intervals, and sudden cardiac death. Circulation. 2007, 115 (4): 442-449. 10.1161/CIRCULATIONAHA.106.668392.PubMed CentralView ArticlePubMedGoogle Scholar
- Catterall WA: Structure and regulation of voltage-gated Ca2+ channels. Annu Rev Cell Dev Biol. 2000, 16: 521-555. 10.1146/annurev.cellbio.16.1.521.View ArticlePubMedGoogle Scholar
- Van Petegem F, et al: Structure of a complex between a voltage-gated calcium channel beta-subunit and an alpha-subunit domain. Nature. 2004, 429 (6992): 671-675. 10.1038/nature02588.PubMed CentralView ArticlePubMedGoogle Scholar
- Maltez JM, et al: Essential Ca(V)beta modulatory properties are AID-independent. Nat Struct Mol Biol. 2005, 12 (4): 372-377. 10.1038/nsmb909.View ArticlePubMedGoogle Scholar
- Leroy J, et al: Interaction via a key tryptophan in the I-II linker of N-type calcium channels is required for beta1 but not for palmitoylated beta2, implicating an additional binding site in the regulation of channel voltage-dependent properties. J Neurosci. 2005, 25 (30): 6984-6996. 10.1523/JNEUROSCI.1137-05.2005.View ArticlePubMedGoogle Scholar
- Bannister JP, et al: Ca(V)1.2 channel N-terminal splice variants modulate functional surface expression in resistance size artery smooth muscle cells. J Biol Chem. 2011, 286 (17): 15058-15066. 10.1074/jbc.M110.182816.PubMed CentralView ArticlePubMedGoogle Scholar
- Tang ZZ, et al: Transcript scanning reveals novel and extensive splice variations in human l-type voltage-gated calcium channel, Cav1.2 alpha1 subunit. J Biol Chem. 2004, 279 (43): 44335-44343. 10.1074/jbc.M407023200.View ArticlePubMedGoogle Scholar
- Wielowieyski PA, et al: Alternative splicing in intracellular loop connecting domains II and III of the alpha 1 subunit of Cav1.2 Ca2+ channels predicts two-domain polypeptides with unique C-terminal tail. J Biol Chem. 2001, 276 (2): 1398-1406. 10.1074/jbc.M006868200.View ArticlePubMedGoogle Scholar
- Buraei Z, Yang J: The Beta subunit of voltage-gated Ca2+ channels. Physiol Rev. 2010, 90 (4): 1461-1506. 10.1152/physrev.00057.2009.PubMed CentralView ArticlePubMedGoogle Scholar
- Napolitano C, Antzelevitch C: Phenotypical manifestations of mutations in the genes encoding subunits of the cardiac voltage-dependent L-type calcium channel. Circ Res. 2011, 108 (5): 607-618. 10.1161/CIRCRESAHA.110.224279.PubMed CentralView ArticlePubMedGoogle Scholar
- Giudicessi JR, et al: Transient outward current (I(to)) gain-of-function mutations in the KCND3-encoded Kv4.3 potassium channel and Brugada syndrom. Heart Rhythm. 2011, 8 (7): 1024-1032. 10.1016/j.hrthm.2011.02.021.PubMed CentralView ArticlePubMedGoogle Scholar
- Schulze-Bahr E, et al: Sodium channel gene (SCN5A) mutations in 44 index patients with Brugada syndrome: different incidences in familial and sporadic disease. Hum Mutat. 2003, 21 (6): 651-652.View ArticlePubMedGoogle Scholar
- David LS, et al: Splice-variant changes of the Ca(V)3.2 T-type calcium channel mediate voltage-dependent facilitation and associate with cardiac hypertrophy and development. Channels (Austin). 2010, 4 (5): 375-389.View ArticleGoogle Scholar
- Adams PJ, et al: Ca(V)2.1 P/Q-type calcium channel alternative splicing affects the functional impact of familial hemiplegic migraine mutations: implications for calcium channelopathies. Channels (Austin). 2009, 3 (2): 110-121.View ArticleGoogle Scholar
- Kobrinsky E, et al: Differential role of the alpha1C subunit tails in regulation of the Cav1.2 channel by membrane potential, beta subunits, and Ca2+ ions. J Biol Chem. 2005, 280 (13): 12474-12485.View ArticlePubMedGoogle Scholar
- Fang K, Colecraft HM: Mechanism of auxiliary β-subunit-mediated membrane targeting of L-type (Cav1.2) channels. J Physiol. 2011, 589: 4437-4455.PubMed CentralView ArticlePubMedGoogle Scholar
- Blumenstein Y, et al: A novel long N-terminal isoform of human L-type Ca2+ channel is up-regulated by protein kinase C. J Biol Chem. 2002, 277 (5): 3419-3423. 10.1074/jbc.C100642200.View ArticlePubMedGoogle Scholar
- Ertel EA, et al: Nomenclature of voltage-gated calcium channels. Neuron. 2000, 25 (3): 533-535. 10.1016/S0896-6273(00)81057-0.View ArticlePubMedGoogle Scholar
- Altier C, et al: Trafficking of L-type calcium channels mediated by the postsynaptic scaffolding protein AKAP79. J Biol Chem. 2002, 277 (37): 33598-33603. 10.1074/jbc.M202476200.View ArticlePubMedGoogle Scholar
- Bichet D, et al: The I-II loop of the Ca2+ channel alpha1 subunit contains an endoplasmic reticulum retention signal antagonized by the beta subunit. Neuron. 2000, 25 (1): 177-190. 10.1016/S0896-6273(00)80881-8.View ArticlePubMedGoogle Scholar
- Snutch TP, et al: Distinct calcium channels are generated by alternative splicing and are differentially expressed in the mammalian CNS. Neuron. 1991, 7 (1): 45-57. 10.1016/0896-6273(91)90073-9.View ArticlePubMedGoogle Scholar
- Altier C, et al: The Cavbeta subunit prevents RFP2-mediated ubiquitination and proteasomal degradation of L-type channels. Nat Neurosci. 2011, 14 (2): 173-180. 10.1038/nn.2712.View ArticlePubMedGoogle Scholar
- Cordeiro JM, et al: Accelerated inactivation of the L-type calcium current due to a mutation in CACNB2b underlies Brugada syndrome. J Mol Cell Cardiol. 2009, 46 (5): 695-703. 10.1016/j.yjmcc.2009.01.014.PubMed CentralView ArticlePubMedGoogle Scholar
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