- Original Paper
- Open Access
Membrane current evoked by mitochondrial Na+–Ca2+ exchange in mouse heart
The Journal of Physiological Sciences volume 70, Article number: 24 (2020)
The electrogenicity of mitochondrial Na+–Ca2+ exchange (NCXm) had been controversial and no membrane current through it had been reported. We succeeded for the first time in recording NCXm-mediated currents using mitoplasts derived from mouse ventricle. Under conditions that K+, Cl−, and Ca2+ uniporter currents were inhibited, extra-mitochondrial Na+ induced inward currents with 1 μM Ca2+ in the pipette. The half-maximum concentration of Na+ was 35.6 mM. The inward current was diminished without Ca2+ in the pipette, and was augmented with 10 μM Ca2+. The Na+-induced inward currents were largely inhibited by CGP-37157, an NCXm blocker. However, the reverse mode of NCXm, which should be detected as an outward current, was hardly induced by extra-mitochondrial application of Ca2+ with Na+ in the pipette. It was concluded that NCXm is electrogenic. This property may be advantageous for facilitating Ca2+ extrusion from mitochondria, which has large negative membrane potential.
Mitochondrial Ca2+ has pivotal roles in mitochondrial metabolism, apoptosis, and cytoplasmic Ca2+ signaling [1,2,3,4,5]. Mitochondrial Ca2+ influx is mainly mediated via mitochondrial Ca2+ uniporter (MCU), and efflux via Na+–Ca2+ exchanger (NCXm) and H+–Ca2+ exchanger. MCU is a Ca2+ channel, whose flux is driven by the negative mitochondrial membrane potential (ΔΨ), − 180 mV, as demonstrated in the patch clamp experiments using mitoplasts . H+–Ca2+ exchanger is likely to be electroneutral, exchanging two H+ with one Ca2+ . However, the electrophysiological property of NCXm has been unknown.
Carafoli et al. first discovered NCXm , namely Na+-dependent mitochondrial Ca2+ efflux, in rat heart, and Palty et al. identified NCLX as an essential component of NCXm . Since the study by Palty et al. , physiological significances of NCLX or NCXm have been extensively elucidated in many types of cell, such as automaticity of cultured cardiomyocytes , insulin secretion of pancreatic β cells [10, 11], control of nociceptive signaling in dorsal root ganglion neurons , B cell receptor-mediated Ca2+ signaling and chemotaxis of B lymphocytes [13,14,15], and Ca2+ oscillation in depolarized mitochondria of mast cells . The tamoxifen-induced knockout of NCLX in mouse heart resulted in severe myocardial dysfunction and heart failure . In addition, it was reported that NCLX is associated with a familial form of Parkinson’s disease where PINK-1 deficiency leads to impairment of mitochondrial Ca2+ efflux  and also with a progression of Alzheimer’s disease . Despite the importance of NCXm in physiological and pathophysiological cell functions, its dependence on ΔΨ, which is the key biophysical property for mitochondrial ATP synthesis, has been controversial.
Early studies using fluorescence probes and Ca2+-sensitive electrode suggested that NCXm activity depends on ΔΨ, based on findings of a high Hill coefficient for cytoplasmic Na+ (∼ 3) and the attenuation of Na+-dependent Ca2+ efflux by mitochondrial depolarization in rat heart mitochondria [20, 21]. Jung et al. later supported the ΔΨ-dependence of NCXm by showing the disruption of Ca2+ efflux through NCXm by dissipation of ΔΨ in beef heart mitochondria . To the contrary, other studies suggested electroneutral exchange via NCXm. Affolter and Carafoli demonstrated that ΔΨ did not alter when the Ca2+ efflux via NCXm was induced using rat heart mitochondria . Brand  and Wingrove and Gunter  supported this idea by showing a Hill coefficient of two for Na+ using rat heart and liver mitochondria, respectively. Later, using imaging methods, we demonstrated the reversal of NCXm activity by ΔΨ depolarization and NCXm activity-dependent change of ΔΨ in permeabilized rat cardiomyocytes, and suggested that NCXm is voltage dependent and electrogenic . Dash and Beard also supported the electrogenic property with a stoichiometry of 3:1 by comparing simulation results of a mathematical model of mitochondria with NCXm of 3:1 or 2:1 stoichiometry to the experimental data . The controversy has been caused by difficulty in direct measurement of membrane current through NCXm. Here we succeeded, for the first time, in recording and characterizing the NCXm-mediated current using mitoplasts derived from mouse heart.
C57BL/6J mice were housed in a 12 h light–dark cycle with ad libitum access to food and water. The experimental protocols were approved by Animal Research Committee, University of Fukui.
Isolation of mouse ventricular mitochondria by differential centrifugation
10–16 week old C57BL/6J mice were heparinized (200 U/mouse, i.p.) and sacrificed by cervical dislocation. The ventricular mitochondria were isolated by a conventional differential centrifugation method. The heart was quickly excised after thoracotomy and placed on an ice-cold sucrose buffer with 0.05% bovine serum albumin (BSA), and the atria and other debris were removed to isolate the ventricular tissues. The ventricular tissue was then cut into pieces and homogenized in the sucrose buffer with 0.05% BSA. The homogenate was centrifuged for 10 min at 8500g. The pellet was re-suspended in the sucrose buffer with 0.05% BSA, and centrifuged for 10 min at 800g. The resulting pellet contains nucleus and unbroken cells. To collect the mitochondria, the supernatant was centrifuged for 10 min at 8500g, washed with the sucrose buffer without BSA, and the resulting pellet which contains mitochondria was re-suspended in 100 μl sucrose buffer without BSA and stored on ice. The sucrose buffer contained 250 mM sucrose, 5 mM HEPES, and 1 mM EGTA (pH 7.2 with KOH). All centrifugation steps were performed at 2 °C.
Western blot analysis
Isolated mitochondria (25 μg) were lysed with a Laemmli sample buffer (Bio-Rad) containing β-mercaptoethanol, denatured at 55 °C for 30 min, resolved by SDS-PAGE and transferred to PVDF membranes (Bio-Rad). Blots were incubated for 1 h at room temperature in blocking one (Nacalai tesque), then incubated in primary antibodies, anti-MCU (Cell Signaling Technology; 1:1000) or anti-COX IV (abcam; 1:2000) for 1 h. Blots were incubated with HRP-linked 2nd antibodies for 30 min. The images were developed with ECL Prime Western Blotting Detection Reagent (GE Healthcare) and acquired by ChemiDoc XRS Plus (Bio-Rad).
Isolated mitochondria were centrifuged for 10 min at 8500g. The pellet was given hypotonic shock for 5 min to yield mitoplasts. The mitoplasts were collected by centrifugation for 5 min at 8500g. The pellet was suspended in a storage buffer. The entire procedure was performed on ice and ice-cold solutions were used. The mitoplast suspension was stored on ice and used within 4–5 h. The hypotonic solution contained 5 mM sucrose, 5 mM HEPES, and 1 mM EGTA (pH 7.2 with KOH), and the storage buffer contained 750 mM KCl, 100 mM HEPES, and 1 mM EGTA (pH 7.2 with KOH).
Labeling of mitochondria and confocal imaging
The isolated mitochondria were loaded with 2 μM MitoTracker Green FM (ThermoFisher Scientific) for 1 h on ice. The confocal images were taken using a confocal microscope with a ×100 objective lens with the excitation at 473 nm and the emission at 485–585 nm (Olympus FV1200).
Ca2+ uptake assay
For measurement of extra-mitochondrial Ca2+, isolated mitochondria (75 μg) were suspended in an assay buffer (100 μl) containing 125 mM KCl, 2 mM K2HPO4, 20 mM HEPES, 0.01 mM EGTA, 2 mM MgCl2, 1 mM malate, 7 mM potassium pyruvate, 5 μM cyclosporin A (Sigma-Aldrich), and 0.5 μM Calcium Green-5N (pH 7.2 with KOH), then were placed in 96-well plate. The extra-mitochondrial Ca2+ was evaluated by measuring fluorescence using a multimode plate reader (Enspire, PerkinElmer), with the excitation at 505 nm and the emission at 530 nm. At 410 s, mitochondria were challenged by 50 μM CaCl2 in the presence or absence of 25 mM NaCl, to initiate Ca2+ influx into mitochondria via MCU. At 1000 s, an MCU blocker, 5 μM Ru360 (Calbiochem), was added to facilitate Ca2+ efflux from mitochondria. The initial Ca2+ efflux velocity was calculated by fitting linearly to the data for initial 60 s after the addition of Ru360.
For measurement of intra-mitochondrial Ca2+, isolated mitochondria (50 μg) were loaded with 20 μM Fluo-8, AM (AAT Bioquest) for 30 min at 25 °C, followed by washing twice. The resulting mitochondria in assay buffer (200 μl) containing 125 mM KCl, 2 mM K2HPO4, 20 mM HEPES, 0.01 mM EGTA, 2 mM MgCl2, 1 mM malate, 7 mM potassium pyruvate, and 5 μM cyclosporin A (pH 7.2 with KOH) were placed in 96-well plate. The intra-mitochondrial Ca2+ was evaluated by measuring fluorescence with the excitation at 490 nm and the emission at 514 nm. At 300 s, mitochondria were challenged by 20 μM CaCl2 in the presence or absence of 5 μM Ru360 or 10 μM ruthenium red (Wako), to initiate Ca2+ influx into mitochondria via known Ca2+ influx systems including MCU. The initial Ca2+ influx velocity was calculated by fitting linearly to the data for initial 26 s after the addition of 20 μM CaCl2.
To induce exchange of intra-mitochondrial Na+ with extra-mitochondrial Ca2+, i.e., reverse mode of NCXm, the Fluo-8, AM loading procedure was performed in the presence of a Na+ ionophore 4 μM monensin and of a Na+–H+ antiporter blocker 100 μM ethylisopropyl amiloride (EIPA; Tocris Biosciences) in Mg2+-free assay buffer where 125 mM KCl was replaced with 125 mM NaCl to facilitate mitochondrial Na+ accumulation. The resulting mitochondria were re-suspended in assay buffer (200 μl) containing 125 mM KCl, 25 mM Na+, 2 mM K2HPO4, 20 mM HEPES, 0.01 mM EGTA, 2 mM MgCl2, 1 mM malate, 7 mM potassium pyruvate, 100 μM EIPA, 10 μM ruthenium red, and 5 μM cyclosporin A (pH 7.2 with KOH). Since mitochondrial depolarization facilitated reverse mode of NCXm , 10 μM antimycin A (Sigma-Aldrich) and 2 μM oligomycin (Sigma-Aldrich) were also added. To evaluate intra-mitochondrial Na+-induced extra-mitochondrial Ca2+ influx, the same protocol was performed in the absence of Na+ throughout the experiment for comparison. The initial Ca2+ influx velocity was calculated by fitting linearly to the data for initial 26 s after the addition of 20 μM CaCl2.
A perfusion chamber was equipped on an inverted microscopy (TE2000-U, Nikon) with a ×100 objective lens. The glass bottom of chamber was pre-treated for 5 min with a KCl-divalent free (KCl-DVF) solution containing 0.05% BSA, to prevent adhesion of mitoplasts. The mitoplast suspension of 3–5 μl was added to 35 μl of the KCl-DVF solution on the bottom of chamber. Solitary mitoplasts with a diameter of ~ 2–3 μm and with round shape were selected for whole-mitoplast patch. The mitoplasts were initially perfused with the KCl-DVF solution. Bath solution was changed within 5 s using a perfusion controller (Valvelink-8.2, Automate scientific). The KCl-DVF solution contained 150 mM KCl, 10 mM HEPES, and 1 mM EGTA (pH 7.2 with KOH).
Voltage clamp experiment was performed using a patch clamp amplifier (Axopatch 200B, Molecular Devices), a digitizer (Digidata 1440A, Molecular Devices) and a software (pClamp 10.7, Molecular Devices). All data were sampled at 10 kHz and later filtered at 2 kHz. For graphical presentation, the membrane current traces were further filtered at 500 Hz (Gaussian filter). Pipettes were prepared using a puller (PC-100, Narishige). After the formation of GΩ seal, the capacitance was compensated and voltage pulses of 350–700 mV for 5–10 ms duration were applied to rupture the membrane and to form the whole mitoplast configuration. The capacitance of mitoplast was 0.1–1.0 pF (0.32 ± 0.22 pF, n = 34). The membrane potential was held at 0 mV, and the ramp pulse of 900 ms duration from −160 to 80 mV was applied every 10 s.
To measure the Na+-induced inward NCXm current, a Na+-free and Ca2+-containing pipette solution was used, and the bath solution was changed from a Na+-free and Ca2+-free bath solution to a Na+-containing bath solution. The Na+-free and Ca2+-containing pipette solution contained 30 mM tetramethylammonium hydroxide (TMA-OH), 2 mM HCl, 100 mM HEPES, and 1.5 mM EGTA. 0, 1.038 and 1.5 mM CaCl2 were added to get 0, 1 and 10 μM free Ca2+, respectively (pH 7.2 with d-gluconic acid). The free Ca2+ concentration was calculated with an online calculator, WEBMAXC standard (https://somapp.ucdmc.ucdavis.edu/pharmacology/bers/maxchelator/webmaxc/webmaxcS.htm). The pipette resistance was 30–40 MΩ when filled with the pipette solution. The Na+-free and Ca2+-free bath solution contained 145 mM HEPES, 50 mM Tris, and 5 mM EGTA (pH 7.2 with Tris). The Na+-containing bath solution contained 145 mM HEPES, 50 mM NaOH, and 5 mM EGTA (pH 7.2 with Tris).
To measure the Ca2+-induced outward Na+–Ca2+ exchange current, a Na+-containing pipette solution was used; 30 mM TMA-OH, 100 mM NaOH, 2 mM HCl, 100 mM HEPES, 1.5 mM EGTA, and 0.6058 mM CaCl2 (pH 7.5 with d-gluconic acid). Calculated free Ca2+ concentration was 0.1 μM. A Ca2+-free bath solution contained 145 mM HEPES, 30 mM Tris, 20 mM NaOH, 5 mM EGTA, and 3.2 mM HCl (pH 7.2 with HEPES). Composition of 1 mM Ca2+-containing bath solution was 145 mM HEPES, 30 mM Tris, 20 mM NaOH, 1.2 mM HCl, 0 mM EGTA, and 1 mM CaCl2 (pH 7.2 with HEPES).
To block the mitochondrial Ca2+ uniporter, 1 μM Ru360 was added to all the bath solutions (IC50 of 184 pM ). To block the NCXm, 2 μM CGP-37157 (Tocris Bioscience) was added to the bath solutions (IC50 of 0.36 μM ).
An average of three consecutive membrane currents in response to ramp pulses was used for analysis in each condition. All electrophysiological recordings were performed under continuous perfusion of bath solutions at 22–25 °C.
All data are demonstrated as mean ± s.e.m. of individual experiments which are presented as n. Statistical analyses were performed with unpaired two-tailed Student’s t test for two-group comparisons or with one-way ANOVA multiple comparisons, followed by Student–Newman–Keuls Method, respectively, using SigmaPlot 14 (Systat Software, Inc.). p < 0.05 was considered significant.
Quality assessment of mitochondria
We first examined the quality of the isolated mitochondria. Western blot analysis confirmed the expression of mitochondrial proteins, MCU and COX IV, in the preparations (Fig. 1a). The quality of mitoplast was evaluated using MitoTracker Green-loaded mitochondria (Fig. 1b). The transmit image of a mitoplast clearly showed the inner mitochondrial membrane as a circle and the remnants of ruptured outer mitochondrial membrane. The fluorescent and merged images of mitoplasts confirmed that the mitoplast originated from mitochondria.
Mitochondrial Ca2+ uptake and extrusion were evaluated by monitoring extra-mitochondrial Ca2+ with Calcium Green 5N (Fig. 2a). An addition of 50 μM Ca2+ caused a transient rise and subsequent decline of extra-mitochondrial Ca2+, suggesting Ca2+ uptake by MCU. The following addition of Ru360, an inhibiter of MCU, induced Ca2+ efflux, which had two components, extra-mitochondrial Na+-dependent and -independent. The Na+-dependent Ca2+ efflux was defined as NCXm and its Ca2+ transporting rate was about 1.5-fold larger than that of Na+-independent Ca2+ efflux (Fig. 2b). The results confirm that NCXm does exist in mouse ventricular mitochondria.
Na+-induced inward current
The membrane currents were first measured using square pulses with a holding potential of 0 mV changing to − 160 ∼ + 40 mV every 20 mV with no Na+ and 1 μM Ca2+ in the pipette solution. An application of extra-mitochondrial 50 mM Na+ augmented the amplitude of inward currents (a middle panel vs a left panel of Fig. 3a). The difference currents between those in the presence and absence of Na+ demonstrated Na+ induced-inward currents, which are time-independent (a right panel of Fig. 3a). The summarized current–voltage relations are shown in Fig. 3b, c, demonstrating Na+-induced inward currents at all membrane potentials examined (Fig. 3c). Since the Na+-induced current was time-independent, we employed a ramp voltage protocol of 900 ms duration. The ramp voltage protocol demonstrated Na+-induced inward currents essentially similar to those with the square pulse protocol (Fig. 3d, e). In the following experiments, we employed the ramp voltage pulse protocol.
Inhibition of Na+-induced inward current by CGP-37157
Next, we examined the effects of CGP-37157, a well-known NCXm blocker, on the Na+-induced inward current. 2 μM CGP-37157 significantly blocked the Na+-induced inward current by 67% (Fig. 4a, b), suggesting the current was mediated by NCXm, at least in part.
It has been recognized that NCXm is able to operate exchange of Li+ with Ca2+ [8, 20], unlike the plasma membrane Na+–Ca2+ exchange. Consistent with the unique property, 50 mM Li+ induced inward currents which were comparable to the Na+-induced inward current with a lower magnitude (Fig. 4c, d). CGP-37157 blocked the Li+-induced current by 74%, similarly to the Na+-induced current (Fig. 4b, d). These data suggested that the Na+- or Li+-induced inward current was mediated by NCXm.
Na+ and Ca2+ concentration dependences of Na+-induced current
Extra-mitochondrial Na+ dependence was examined in Fig. 5a, b. The current was clearly dependent on extra-mitochondrial Na+ concentration, with a half-maximum concentration of 35.6 mM. We further studied intra-mitochondrial Ca2+ dependence by altering the Ca2+ concentration in the pipette solution. Without Ca2+ in the pipette solution, the application of 50 mM Na+ hardly induced inward current. Conversely, with 10 μM Ca2+ in the pipette solution, the Na+-induced current markedly increased (Fig. 5c, d).
Ca2+-induced outward current
It was reported that NCXm could operate in a reverse mode, i.e. Ca2+ uptake in exchanging with mitochondrial Na+ [16, 22, 26, 30, 31]. We tried to detect outward current by applying extra-mitochondrial Ca2+ with high-concentration Na+ in the pipette (100 mM). Contrary to our expectation, extra-mitochondrial Ca2+, up to 1 mM, hardly evoked outward current (Fig. 6).
To explore reasons why the outward NCXm current was not detectable, we evaluated Ca2+ uptake via the reverse mode of NCXm by measuring intra-mitochondrial Ca2+ using Fluo-8. In the mitochondria loaded with Na+, an application of 20 μM Ca2+ under the condition of mitochondrial depolarization induced a slow increase in intra-mitochondrial Ca2+, whose rate was only 1.6 times faster than that of Na+-unloaded mitochondria (Fig. 7a, b). The slow Ca2+ rise was blocked by 2 μM CGP-37157, suggesting that the Ca2+ rise was mediated via the reverse mode of NCXm (Fig. 7a, b). Contrarily, the rate of Ca2+ uptake though known Ca2+ influx systems including MCU under the condition of normal ΔΨ was larger by an order of magnitude than that of the reverse mode of NCXm; Ru360 and ruthenium red-sensitive Ca2+ uptake rate was 208.7 ± 11.8 A.U./s and 219.9 ± 11.6, respectively (Fig. 7c, d), and CGP-37157-sensitive Na+-dependent Ca2+ uptake rate was 6.7 ± 0.4 A.U./s (n = 4) (Fig. 7a, b). The slower turnover of reverse mode of NCXm may hamper recording of membrane current mediated by the reverse mode of NCXm.
In this study, we report, for the first time, the membrane current mediated by NCXm using the whole-mitoplast patch clamp technique. The recorded inward current is most likely mediated by the NCXm based on the Na+ and Li+ selectively, the requirement of Ca2+ in the opposite membrane site, and the inhibition by CGP-37157. This study provides a final conclusion on the electrogenicity of NCXm which has been controversial for long time [20,21,22,23,24,25,26,27].
A variety of half-maximum concentration values of NCXm for extra-mitochondrial Na+ has been reported in cardiac myocytes and other cells, ranging from 0.9 to 12 mM [11, 20, 25, 26]. The half-maximum concentration of 35.6 mM, derived from the present study, is rather high. This might be partly because contamination of Na+-permeable current could not be completely eliminated under our conditions. Further detailed examinations for clarifying the origin of Na+-leak currents are necessary to solve the problem. Nevertheless, the cytosolic Na+ dependence of NCXm may have an important role under the conditions of heart failure, in which situation both cytosolic Ca2+ and Na+ tend to increase [32,33,34]. The rise of cytosolic Ca2+ may induce mitochondrial Ca2+ overload and dysfunction. However, the elevation of cytosolic Na+ may facilitate mitochondrial Ca2+ efflux through NCXm and protect mitochondrial dysfunction .
The stoichiometry of NCXm is an important issue. The fact that the exchange of extra-mitochondrial Na+ with intra-mitochondrial Ca2+ produces inward current indicates the stoichiometry 3 or more Na+:1 Ca2+ exchange. However, it was not possible to derive it from reversal potentials because of the relatively small current density and the difficulty in inducing the outward current. The reverse mode of NCXm was described earlier [16, 22, 26, 30, 31]. However, the mitochondrial Ca2+ rise through the reverse mode of NCXm was relatively slow and it took more than several tens of minutes to reach a steady state . Consistent with the previous observation, the intra-mitochondrial Ca2+ rise though reverse mode of NCXm was much slower than that of MCU (Fig. 7). It should be noted that the rate of extra-mitochondrial Ca2+ change through the forward mode of NCXm is in a level comparable to that of MCU (Fig. 2). Therefore, it may be reasonable to speculate that the operation of reverse mode of NCXm is much slower than the forward mode. NCXm might go into an inactivated state at higher intra-mitochondrial Na+ concentrations, in a similar manner to plasma membrane NCX . A method for faster ion concentration jump, which was used for NCX current study, may be useful for studying the possible inactivation, but it could not be used in this study because of relatively fragile nature of mitoplast. Further study is needed to clarify the mechanisms of slower operation of reverse mode and to determine the stoichiometry.
In this study, we used CGP-37157 at a sub-saturating concentration, 2 μM, in the electrophysiological experiments to avoid its possible off-target effects. It has been reported that CGP-37157 affects many ion channels and transporters including plasma membrane Na+–Ca2+ exchange at higher concentrations [37,38,39]. Palty et al. reported that 5 μM CGP-37157 exhibited approximately 50% inhibition of Ca2+ efflux from mitochondria . The effect of 2 μM CGP-37157 on the Na+-induced current (67%) is comparable to the inhibitory effects shown in the previous report. Therefore, the CGP-37157-sensitive current component is most likely to be mediated by NCXm. However, we assume that other membrane currents such as leak current were, at least partially, contaminated when 10 μM Ca2+ was included in the pipette solution because outward current was induced (Fig. 5c).
ΔΨ is about −180 mV with reference to cytosol, and are the energy source for ATP synthesis from ADP and inorganic phosphate by ATP synthase. The ΔΨ strongly facilitates Ca2+ entering into mitochondria through MCU and other Ca2+-permeable systems. The voltage-dependent nature of NCXm is advantageous for Ca2+ extrusion over electroneutral exchange. Therefore, ΔΨ depolarization under the pathological conditions such as ischemia should attenuate both Ca2+ influx and efflux, resulting in severe damage of mitochondria.
The mitochondrial Na+– or Li+–Ca2+ exchange current was identified for the first time in mitoplasts derived from mouse ventricle. It was concluded that NCXm is electrogenic with a stoichiometry of 3 or more Na+:1 Ca2+.
Availability of data and materials
All data generated or analyzed during this study are included in this published article.
Mitochondrial Na+–Ca2+ exchange
Mitochondrial Ca2+ uniporter
Mitochondrial membrane potential
Bovine serum albumin
Bernardi P (1999) Mitochondrial transport of cations: channels, exchangers, and permeability transition. Physiol Rev 79:1127–1155. https://doi.org/10.1152/physrev.1918.104.22.1687
Takeuchi A, Kim B, Matsuoka S (2015) The destiny of Ca2+ released by mitochondria. J Physiol Sci 65:11–24. https://doi.org/10.1007/s12576-014-0326-7
Saito R, Takeuchi A, Himeno Y, Inagaki N, Matsuoka S (2016) A simulation study on the constancy of cardiac energy metabolites during workload transition. J Physiol 594:6929–6945. https://doi.org/10.1113/JP272598
Kostic M, Sekler I (2019) Functional properties and mode of regulation of the mitochondrial Na+/Ca2+ exchanger, NCLX. Semin Cell Dev Biol 94:59–65. https://doi.org/10.1016/j.semcdb.2019.01.009
Takeuchi A, Matsuoka S (2020) Integration of mitochondrial energetics in heart with mathematical modelling. J Physiol. https://doi.org/10.1113/JP276817
Kirichok Y, Krapivinsky G, Clapham DE (2004) The mitochondrial calcium uniporter is a highly selective ion channel. Nature 427:360–364. https://doi.org/10.1038/nature02246
Carafoli E, Tiozzo R, Lugli G, Crovetti F, Kratzing C (1974) The release of calcium from heart mitochondria by sodium. J Mol Cell Cardiol 6:361–371. https://doi.org/10.1016/0022-2828(74)90077-7
Palty R, Silverman WF, Hershfinkel M, Caporale T, Sensi SL, Parnis J, Nolte C, Fishman D, Shoshan-Barmatz V, Herrmann S, Khananshvili D, Sekler I (2010) NCLX is an essential component of mitochondrial Na+/Ca2+ exchange. Proc Natl Acad Sci U S A 107:436–441. https://doi.org/10.1073/pnas.0908099107
Takeuchi A, Kim B, Matsuoka S (2013) The mitochondrial Na+–Ca2+ exchanger, NCLX, regulates automaticity of HL-1 cardiomyocytes. Sci Rep 3:2766. https://doi.org/10.1038/srep02766
Nita II, Hershfinkel M, Fishman D, Ozeri E, Rutter GA, Sensi SL, Khananshvili D, Lewis EC, Sekler I (2012) The mitochondrial Na+/Ca2+ exchanger upregulates glucose dependent Ca2+ signalling linked to insulin secretion. PLoS ONE 7:e46649. https://doi.org/10.1371/journal.pone.0046649
Nita II, Hershfinkel M, Kantor C, Rutter GA, Lewis EC, Sekler I (2014) Pancreatic beta-cell Na+ channels control global Ca2+ signaling and oxidative metabolism by inducing Na+ and Ca2+ responses that are propagated into mitochondria. FASEB J 28:3301–3312. https://doi.org/10.1096/fj.13-248161
Nita II, Caspi Y, Gudes S, Fishman D, Lev S, Hersfinkel M, Sekler I, Binshtok AM (2016) Privileged crosstalk between TRPV1 channels and mitochondrial calcium shuttling machinery controls nociception. Biochim Biophys Acta 1863:2868–2880. https://doi.org/10.1016/j.bbamcr.2016.09.009
Kim B, Takeuchi A, Koga O, Hikida M, Matsuoka S (2012) Pivotal role of mitochondrial Na+–Ca2+ exchange in antigen receptor mediated Ca2+ signalling in DT40 and A20 B lymphocytes. J Physiol 590:459–474. https://doi.org/10.1113/jphysiol.2011.222927
Kim B, Takeuchi A, Hikida M, Matsuoka S (2016) Roles of the mitochondrial Na+–Ca2+ exchanger, NCLX, in B lymphocyte chemotaxis. Sci Rep 6:28378. https://doi.org/10.1038/srep28378
Takeuchi A, Kim B, Matsuoka S (2020) Physiological functions of mitochondrial Na+–Ca2+ exchanger, NCLX, in lymphocytes. Cell Calcium 85:102114. https://doi.org/10.1016/j.ceca.2019.102114
Samanta K, Mirams GR, Parekh AB (2018) Sequential forward and reverse transport of the Na+ Ca2+ exchanger generates Ca2+ oscillations within mitochondria. Nat Commun 9:156. https://doi.org/10.1038/s41467-017-02638-2
Luongo TS, Lambert JP, Gross P, Nwokedi M, Lombardi AA, Shanmughapriya S, Carpenter AC, Kolmetzky D, Gao E, van Berlo JH, Tsai EJ, Molkentin JD, Chen X, Madesh M, Houser SR, Elrod JW (2017) The mitochondrial Na+/Ca2+ exchanger is essential for Ca2+ homeostasis and viability. Nature 545:93–97. https://doi.org/10.1038/nature22082
Kostic M, Ludtmann MH, Bading H, Hershfinkel M, Steer E, Chu CT, Abramov AY, Sekler I (2015) PKA phosphorylation of NCLX reverses mitochondrial calcium overload and depolarization, promoting survival of PINK1-deficient dopaminergic neurons. Cell Rep 13:376–386. https://doi.org/10.1016/j.celrep.2015.08.079
Jadiya P, Kolmetzky DW, Tomar D, Di Meco A, Lombardi AA, Lambert JP, Luongo TS, Ludtmann MH, Pratico D, Elrod JW (2019) Impaired mitochondrial calcium efflux contributes to disease progression in models of Alzheimer’s disease. Nat Commun 10:3885. https://doi.org/10.1038/s41467-019-11813-6
Crompton M, Capano M, Carafoli E (1976) The sodium-induced efflux of calcium from heart mitochondria. A possible mechanism for the regulation of mitochondrial calcium. Eur J Biochem 69:453–462. https://doi.org/10.1111/j.1432-1033.1976.tb10930.x
Crompton M, Kunzi M, Carafoli E (1977) The calcium-induced and sodium-induced effluxes of calcium from heart mitochondria. Evidence for a sodium–calcium carrier. Eur J Biochem 79:549–558. https://doi.org/10.1111/j.1432-1033.1977.tb11839.x
Jung DW, Baysal K, Brierley GP (1995) The sodium–calcium antiport of heart mitochondria is not electroneutral. J Biol Chem 270:672–678. https://doi.org/10.1074/jbc.270.2.672
Affolter H, Carafoli E (1980) The Ca2+–Na+ antiporter of heart mitochondria operates electroneutrally. Biochem Biophys Res Commun 95:193–196. https://doi.org/10.1016/0006-291x(80)90723-8
Brand MD (1985) The stoichiometry of the exchange catalysed by the mitochondrial calcium/sodium antiporter. Biochem J 229:161–166. https://doi.org/10.1042/bj2290161
Wingrove DE, Gunter TE (1986) Kinetics of mitochondrial calcium transport. II. A kinetic description of the sodium-dependent calcium efflux mechanism of liver mitochondria and inhibition by ruthenium red and by tetraphenylphosphonium. J Biol Chem 261:15166–15171
Kim B, Matsuoka S (2008) Cytoplasmic Na+-dependent modulation of mitochondrial Ca2+ via electrogenic mitochondrial Na+–Ca2+ exchange. J Physiol 586:1683–1697. https://doi.org/10.1113/jphysiol.2007.148726
Dash RK, Beard DA (2008) Analysis of cardiac mitochondrial Na+–Ca2+ exchanger kinetics with a biophysical model of mitochondrial Ca2+ handling suggests a 3:1 stoichiometry. J Physiol 586:3267–3285. https://doi.org/10.1113/jphysiol.2008.151977
Matlib MA, Zhou Z, Knight S, Ahmed S, Choi KM, Krause-Bauer J, Phillips R, Altschuld R, Katsube Y, Sperelakis N, Bers DM (1998) Oxygen-bridged dinuclear ruthenium amine complex specifically inhibits Ca2+ uptake into mitochondria in vitro and in situ in single cardiac myocytes. J Biol Chem 273:10223–10231. https://doi.org/10.1074/jbc.273.17.10223
Cox DA, Conforti L, Sperelakis N, Matlib MA (1993) Selectivity of inhibition of Na+–Ca2+ exchange of heart mitochondria by benzothiazepine CGP-37157. J Cardiovasc Pharmacol 21:595–599. https://doi.org/10.1097/00005344-199304000-00013
Griffiths EJ (1999) Reversal of mitochondrial Na/Ca exchange during metabolic inhibition in rat cardiomyocytes. FEBS Lett 453:400–404. https://doi.org/10.1016/s0014-5793(99)00726-7
Smets I, Caplanusi A, Despa S, Molnar Z, Radu M, VandeVen M, Ameloot M, Steels P (2004) Ca2+ uptake in mitochondria occurs via the reverse action of the Na+/Ca2+ exchanger in metabolically inhibited MDCK cells. Am J Physiol Renal Physiol 286:F784–F794. https://doi.org/10.1152/ajprenal.00284.2003
Murphy E, Eisner DA (2009) Regulation of intracellular and mitochondrial sodium in health and disease. Circ Res 104:292–303. https://doi.org/10.1161/Circresaha.108.189050
Despa S, Bers DM (2013) Na+ transport in the normal and failing heart—remember the balance. J Mol Cell Cardiol 61:2–10. https://doi.org/10.1016/j.yjmcc.2013.04.011
Santulli G, Xie WJ, Reiken SR, Marks AR (2015) Mitochondrial calcium overload is a key determinant in heart failure. Proc Natl Acad Sci USA 112:11389–11394. https://doi.org/10.1073/pnas.1513047112
Liu T, O’Rourke B (2008) Enhancing mitochondrial Ca2+ uptake in myocytes from failing hearts restores energy supply and demand matching. Circ Res 103:279–288. https://doi.org/10.1161/CIRCRESAHA.108.175919
Hilgemann DW, Matsuoka S, Nagel GA, Collins A (1992) Steady-state and dynamic properties of cardiac sodium–calcium exchange. Sodium-dependent inactivation. J Gen Physiol 100:905–932. https://doi.org/10.1085/jgp.100.6.905
Czyz A, Kiedrowski L (2003) Inhibition of plasmalemmal Na+/Ca2+ exchange by mitochondrial Na+/Ca2+ exchange inhibitor 7-chloro-5-(2-chlorophenyl)-1,5-dihydro-4,1-benzothiazepin-2(3H)-one (CGP-37157) in cerebellar granule cells. Biochem Pharmacol 66:2409–2411. https://doi.org/10.1016/j.bcp.2003.08.024
Neumann JT, Diaz-Sylvester PL, Fleischer S, Copello JA (2011) CGP-37157 inhibits the sarcoplasmic reticulum Ca2+ ATPase and activates ryanodine receptor channels in striated muscle. Mol Pharmacol 79:141–147. https://doi.org/10.1124/mol.110.067165
Drumm BT, Sung TS, Zheng H, Baker SA, Koh SD, Sanders KM (2018) The effects of mitochondrial inhibitors on Ca2+ signalling and electrical conductances required for pacemaking in interstitial cells of Cajal in the mouse small intestine. Cell Calcium 72:1–17. https://doi.org/10.1016/j.ceca.2018.01.003
This work was supported by Takeda Science Foundation (A.T.), The Mochida Memorial Foundation for Medical and Pharmaceutical Research (A.T.), and JSPS KAKENHI grants; 18K06869 (A.T.), 19H03400 (S. M.), and 19K22509 (S. M.).
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Islam, M.M., Takeuchi, A. & Matsuoka, S. Membrane current evoked by mitochondrial Na+–Ca2+ exchange in mouse heart. J Physiol Sci 70, 24 (2020). https://doi.org/10.1186/s12576-020-00752-3
- Na+–Ca2+ exchange