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Mitochondrial Ca2+ uptake controls actin cytoskeleton dynamics during cell migration

Scientific Reports volume 6, Article number: 36570 (2016) | Download Citation

Abstract

Intracellular Ca2+ signaling regulates cell migration by acting on cytoskeleton architecture, cell directionality and focal adhesions dynamics. In migrating cells, cytosolic Ca2+ pool and Ca2+ pulses are described as key components of these effects. Whereas the role of the mitochondrial calcium homeostasis and the Mitochondria Cacium Uniporter (MCU) in cell migration were recently highlighted in vivo using the zebrafish model, their implication in actin cystokeleton dynamics and cell migration in mammals is not totally characterized. Here, we show that mcu silencing in two human cell lines compromises their migration capacities. This phenotype is characterized by actin cytoskeleton stiffness, a cell polarization loss and an impairment of the focal adhesion proteins dynamics. At the molecular level, these effects appear to be mediated by the reduction of the ER and cytosolic Ca2+ pools, which leads to a decrease in Rho-GTPases, RhoA and Rac1, and Ca2+-dependent Calpain activites, but seem to be independent of intracellular ATP levels. Together, this study highlights the fundamental and evolutionary conserved role of the mitochondrial Ca2+ homeostasis in cytoskeleton dynamics and cell migration.

Introduction

Cell migration contributes to a number of physiological processes including embryonic development, wound healing and immune response. Abnormal cell migration is often associated with cancer progression and invasion1. Cell migration is regulated by external signals and internal factors, including actin cytoskeleton remodeling and regulation of the focal adhesion proteins (FAPs), which participate in key interactions with the extracellular matrix and the cytoskeleton2,3. Intracellular forces generated by FAPs allow the rear-to-front retraction and assembly of actin protrusions, allowing the cell to move4. The turnover of FAPs is spatiotemporally finely controlled by intracellular Ca2+ signaling. Indeed, cell retraction is regulated by the Rho GTPases-dependent actomyosin contraction5,6 and FAPs disassembly7,8, both processes being Ca2+-dependent. Actomyosin contraction is controlled by the phosphorylation of Myosin-Light Chain (MLC) by the Ca2+-Calmodulin MLC kinase pathway9,10, whereas the Ca2+-dependent proteases Calpains are involved in FAPs disassembly7,11,12.

Mitochondria have a central role in the control of the intracellular Ca2+ levels and signaling; they constantly uptake Ca2+ ions under physiological conditions, to ensure their proper functions13. These organelles can rapidly uptake substantial amounts of Ca2+ though the existence of Ca2+ hot spots localized at the interface between the mitochondria and the endoplasmic reticulum (ER)14. The mitochondrial Ca2+ uptake capacities have been also linked to an efficient Store-Operated Ca2+ Entry (SOCE)15,16,17,18. Interestingly, the role of the SOCE process, which is regulated in part by the ER-resident Stromal Interacting Molecule 1 (STIM1) and Calcium release-activated calcium channel protein 1 (Orai1), has been highlighted in the actomyosin contractility19,20 and breast tumor cell migration21.

Recent characterization of the mitochondrial Ca2+ uptake machinery, including the mitochondrial Ca2+ uniporter (MCU)22,23 and associated regulators24,25,26, shed new light on the molecular mechanisms underlying mitochondrial Ca2+ buffering and homeostasis. Although the phenotype of the MCU knock-out (KO) mice is mild27, tissue-specific KOs28,29,30,31 as well as genetic manipulations of mcu in other animal models32,33,34 provided evidence for different physiological functions of MCU35. Using zebrafish as a model, we recently demonstrated that MCU is involved in the control of the first embryonic cell movements32. Indeed mcu silencing led to profound migration defects in the pluripotent stem cells, thus altering anteroposterior axis formation. Subsequent studies on MCU and MICU1 in mammalian cells showed an evolutionarily conserved contribution of the mitochondrial Ca2+ uptake machinery in cell migration. Indeed, in endothelial36 or breast37 and cervical cancer38 cells, alteration of the mitochondrial Ca2+ uptake led to similar defects in migration abilities. Finally, computed data from clinical studies suggested that mcu-overexpression and micu1-under expression were associated with poor prognosis for breast cancer patients38,39. Despite these observations, the downstream molecular actors of this process remain unknown.

Here, we show that silencing mcu gene expression in human breast cancer and HeLa cells led to an actin cytoskeleton stiffness, loss of cell polarity as well as impairment of focal adhesion dynamics. Indeed, the efficient assembly/disassembly of FAPs, including Vinculin and Paxillin, was found to rely on intact mitochondrial Ca2+ uptake. At the molecular level, the effect of mcu silencing appeared to be mediated by a significant decrease of Rho-family GTPases and Calpain activities, as a result of the global decrease of cytosolic and ER Ca2+ pools. Together, our results support a new role of the mitochondrial Ca2+ homeostasis in cytoskeleton dynamics and cell migration.

Results

Mitochondrial Ca2+ uptake is required for efficient cell migration

To investigate the role of the mitochondrial Ca2+ uptake in cell migration, we analyzed the effect of mcu silencing. Two specific short interfering RNAs (siRNAs) were directed to the 3′ UTR region of the mcu transcript, hereafter called si1 and si2 MCU. These siRNAs efficiently decreased the levels of the endogenous MCU protein (Fig. 1a), and led to a significant decrease in the capacity of mitochondria to uptake exogenous Ca2+ (Supplementary Fig. S1a–d). First, in the highly migrating Hs578t breast cancer cell line, we analyzed the effect of mcu silencing on their capacities to close the gap in a classical wound-healing assay. As shown in Fig. 1b,c, mcu knockdown reduced significantly the ability of Hs578t cells to close the wound (43.8% ± 0.7%; 50% ± 1.8% of gap closure for si1 and si2 MCU at 15 hours post wound, respectively) compared to control cells (73.5% ± 0.5% of gap closure). We next examined the capacity of Hs578t cells to migrate through a basement membrane following a serum gradient using a Boyden chamber assay. Compared to control cells, a significantly lower percentage of mcu-silenced cells were found to have crossed the membrane after 7.5 hours (81.9% ± 2.8%; n = 9557 cells counted and 74.2% ± 2.1%; n = 8752 cells counted, for si1 and si2 MCU respectively, compared to 100% for control cells; n = 11728 cells counted) (Fig. 1d,e).

Figure 1: MCU knockdown induces cell migration defects.
Figure 1

(a) Immunoblot blot showing the decrease of MCU protein level in Hs578t cells transfected with two siRNAs (si1 and si2) targeting mcu transcript. Scrambled siRNA (si Control) was used as negative control. Vinculin was used as loading control. Quantitative ratios (MCU expression) between MCU and Vinculin were indicated below. (b) Representative images of the effect of mcu-silencing on Hs578t migration performed by wound healing assay. Compared to control cells, mcu-silenced cells present decreased capacities to close the gap. Scale bar: 200 μm. (c) Histogram representing the percentage of gap closure estimated at 7.5 and 15 hours post-wound from (b) (mean ± S.E.M; n = 4 independent experiments). N.S. = not significant; ***P < 0.001. (d) Representative Grayscale images of the effect of mcu-knockdown on Hs578t invasion performed with Boyden chamber assay using Fetal Bovine Serum (FBS) as chemoattractant. Compared to controls, less mcu-silenced cells have crossed the membrane. Scale bar: 200 μm. (e) Histogram representing the number of invading cells relative to control condition measured at 7.5 hours post-seeding from (d) (mean ± S.E.M; n = 3 independent experiments). *P < 0.05. (f) Representative single cell tracking experiments highlighting the cell paths (blue lines) of isolated Hs578t (red dots) or HeLa cells (red dots), silenced or not for mcu; acquisition time 24 hours. Compared to control cells, mcu-silenced cells have shorter migration paths. (g) Histogram deduced from the results displayed in (f) representing the distance of cell migration relative to control (mean ± S.E.M; 30 cells in each experiment; n = 3 independent experiments). ***P < 0.001. See also Supplementary Fig. S1.

Finally, we examined the effect of mcu-knockdown by directly tracking individual cells and measuring the total traveled distance (TTD) over a 24-hours period. Mcu knockdown in Hs578t significantly reduced cell migration paths compared to controls. Whereas in control cells TTD reached 240.1 μm ± 38.5 μm (n = 60 cells), mcu-silenced cells showed a decreased migration rate, TTD being lowered to 87.7 μm ± 9.3 μm and 138.5 μm ± 18.3 μm (n = 60 cells) for si1 and si2 MCU Hs578t cells, respectively (Fig. 1f,g). Of note, these results were confirmed in a second cell line, HeLa cells, with lower migration rate (Fig. 1f,g). Interestingly, cells treatment with Ru360, a potent MCU inhibitor, led to a similar cell migration defect, highlighting the specific role of the mitochondrial Ca2+ uptake during cell migration (Supplementary Fig. S1e).

Importantly, the cell migration phenotype was not found to be associated with cell proliferation or apoptotic program defects. Indeed, mcu-silenced Hs578t cells did not show any decrease in cell proliferation or increase in apoptosis (Supplementary Fig. S1f,g). Together, these results support the notion that mitochondrial Ca2+ uptake is required for optimal migration of human cells.

MCU downregulation leads to impaired cell polarization and Rho GTPases activities

To further characterize the effects of mitochondrial Ca2+ uptake reduction on cell migration we analyzed the behavior of individual cells lacking MCU using time-lapse videomicroscopy. To perform these experiments we established stable Hs578t MCU negative cells by infection with lentiviruses encoding short hairpin RNAs (shRNAs) targeting the same regions as si1 and si2 MCU siRNAs. ShMCU expressing clones presented the same migration impairment (Supplementary Fig. S2a,b) and decreased mitochondrial Ca2+ uptake (Supplementary Fig. S2c,d), as siRNAs transfected cells. Cells expressing a control shRNA exhibited, in a coordinated fashion, lamellipodia formation at the leading edge and disassembly of adhesion points at the rear end of the cell body, allowing them to migrate (Fig. 2a). These cells presented a typical forward-to-rear polarization, which was absent in shMCU cells. These morphological changes were quantified by measuring the circularity coefficient of the cells (from 0, to an infinitely elongated polygon, to 1 for a perfect circle). Compared to controls, which showed a circularity coefficient of 0.44 ± 0.21 (n = 34 cells), mcu knockdown cells showed an increased circularity coefficient (0.70 ± 0.22; n = 32 cells and 0.75 ± 0.16; n = 29 cells, for sh1 and sh2 MCU cells, respectively), indicating a more circular shape (Fig. 2b).

Figure 2: Mitochondrial Ca2+ uptake impairment leads to cell polarization defects and decreased small GTPases activities.
Figure 2

(a) Representative transmission images of single cell tracking of Hs578t cells stably expressing shRNA control versus shRNA targeting mcu transcript. Cells expressing the control shRNA have forward-to-rear polarization, which was absent in shMCU cells. Scale bar: 20 μm. (b) Graph representing the quantification of circularity coefficients for sh Control (n = 34 cells), sh1 MCU (n = 32 cells) and sh2 MCU (n = 29 cells) (mean ± S.E.M; three independent experiments). Compared to control cells, shMCU cells present an increased circularity coefficient. ***P < 0.001. (c) Confocal time-lapse images showing the CFP (cyan), Venus (yellow) as well as Venus/CFP ratio (RVenus/CFP) of the RhoA2G biosensor dye following IP3R mobilization using Histamine 100 μM in Hs578t cells. Thrombin was used as positive control for RhoA activation. Ratio was visualized as a heat map using false colors. Images were acquired before and after 1 min treatment with Histamine or Thrombin. Following Histamine treatment, RhoA activation is higher in control cells compared to shMCU cells. Scale bar: 20 μm. (d) Histogram showing the Rmax/R0 ratio following Histamine or Thrombin stimulations in control versus mcu-silenced cells, from (c). (mean ± S.E.M.; 20 cells in each experiment; n = 3 independent experiments). **P < 0.01, ***P < 0.001. (e) Immunoblot showing the deacread Rac1 activation (Act. Rac1) in sh MCU compared to sh control cells. Activated Rac1 in Hs578t cells was purified using PAK1 beads and detected using specific Rac1 antibody. Total Rac1 levels were used to normalize the levels of activated Rac1 (numbers below). See also Supplementary Fig. S2.

Lamellipodia dynamics is under the control of the Rho family of GTPases, including Rac1 and RhoA, which are essential for the formation and retraction of lamellipodia6. We first analyzed the activity of RhoA using Fluorescence Resonance Energy Transfer (FRET)-based biosensor RhoA2G40. RhoA2G activity was calibrated using thrombin, which has previously been shown to activate RhoA41. To measure Ca2+ related RhoA activation we used histamine to induce IP3-dependent Ca2+ release from the ER. In these conditions the amount of activated RhoA was significantly decreased in both shMCU Hs578t clones (RhoA2G Rmax/R0 ratio = 1.26 ± 0.24 and 1.24 ± 0.28 for sh1 and sh2 MCU, respectively; n = 20 cells per condition) compared to the control (RhoA2G Rmax/R0 ratio = 1.84 ± 0.41, n = 20 cells) (Fig. 2c,d). In addition we measured basal Rac1 activation using PAK1-based immunoprecipitation assay. Compared to control cells, sh1 and sh2 MCU clones showed decreased levels of activated Rac1 (Fig. 2e), suggesting that mitochondrial Ca2+ uptake is important for Rac1 and RhoA activation.

Mitochondrial Ca2+ uptake impairment induces cytoskeleton stiffness and focal adhesion dynamics defects

The involvement of Rho GTPases in cell polarity and migration is essentially driven by their control of cytoskeleton organization and dynamics6. We thus analyzed the three major cytoskeleton structures: microtubules, intermediate filaments and microfilaments. The overall organization of the microtubules and intermediate filaments using alpha-Tubulin and Vimentin as markers, respectively, showed no significant difference in mcu-silenced cells, compared to controls (Supplementary Fig. S3). However, profound alterations of central microfilament components, including Myosin-Light Chain (MLC) phosphorylation and F-actin fibers, were detected in the cells lacking MCU. Compared to control cells, mcu-silenced cells presented increased phosphorylation levels of MLC residues Thr18 and Ser19, as shown by immunofluorescence (Fig. 3a) and western blotting (Fig. 3b). The observed cytoskeleton stiffness was correlated to a higher density of the F-actin fibers and actin bundles as detected by phalloidin-rhodamine staining (Fig. 3a,c). In fact, actin bundles attach to extracellular matrix through focal adhesion points (FAPs) to provide the mechanical forces required for adhesion, retraction and efficient migration42. We thus checked the status of FAPs by analyzing the distribution of the Vinculin protein. As shown in Fig. 3c, in shMCU cells, Vinculin mainly accumulated in FAPs, in contrast to control cells where Vinculin localization was more diffuse. In fact, the changes of Vinculin localization in mcu-silenced cells were not linked to a variation in Vinculin protein levels (Fig. 3b), suggesting that it could be rather due to alterations in the dynamics of FAPs formation and disassembly. To test this hypothesis we analyzed FAPs dynamics by monitoring Paxillin-GFP expressing cells with fluorescent time-lapse confocal microscopy. In control cells, Paxillin-GFP staining gradually decreased at the tailing edge, allowing the cells to move forward. However, in shMCU cells, Paxillin-GFP staining remained persistent and became even higher during the 20-min time period of monitoring (Fig. 3d). These observations suggested that the FAPs dynamic and structure in mcu-silenced cells were impaired. Quantification of the number of FAPs per cell as well as size measurement revealed a significant increase of both parameters in mcu-silenced cells (Fig. 3e,f). We further monitored the Paxillin phosphorylation level at Tyr 118. Paxillin phosphorylation is orchestrated by the focal adhesion kinase (FAK) and associated with the assembly and turnover of the adhesions43. Moreover, Phospho-Paxillin provides a docking site for recruitment of other signaling molecules required for cell migration. Interestingly, Paxillin phosphorylation was strongly decreased in shMCU cells, as shown by the Phospho-Paxillin/Total Paxillin ratio (Fig. 3g), corroborating the observed Paxillin-GFP dynamics in live cell imaging. Paxillin turnover in FAPs is controlled by the Ca2+-dependent, non-lysosomal cysteine proteases known as Calpains. We therefore analyzed the effet of mcu silencing on global Calpains activity. As shown in Fig. 3h, Calpains activity showed a 40% decrease in mcu-silenced cells (57.4% ± 18.1% and 59.5% ± 11.7% for sh1 and sh2 MCU respectively, compared to 100% for control cells). Together, these results suggest that mitochondrial Ca2+ uptake, acts on cell migration by controlling F-actin microfilaments and focal adhesion dynamics, in a Calpain-dependent manner.

Figure 3: Mitochondrial Ca2+ uptake is required for cytoskeleton and focal adhesion protein dynamics.
Figure 3

(a) Representative confocal images showing the accumulation of phospho-myosin light chain (P-MLC) signal in F-actin fibers in sh2 MCU cells compared to controls. P-MLC and F-actin were stained using P-MLC antibody and phalloidine rhodamine probe, respectively. Merge channels between P-MLC (green) and F-actin (red) were presented in the rightmost panels. Scale bar: 20 μm. (b) Immunoblot showing the increase of MLC phosphorylation on Serine19 (P-MLC) and Threonine18 and Serine19 (P2-MLC) positions in mcu-silenced cells. MCU antibody was used to show the efficiency of the shRNAs. F1F0 ATPase antibody was used as loading control. (c) Representative confocal images showing the accumulation of Vinculin in FAPs in sh2 MCU cells compared to control. Vinculin and F-actin were detected using anti-Vinculin antibody and phalloidine rhodamine probe, respectively. Merge channels between Vinculin (green) and F-actin (red) were presented in the rightmost panels. Scale bar: 20 μm. (d) Representative time-lapse confocal images showing the persistence of Paxillin-GFP signal in the FAPs of mcu-knockdown cells compared to control. Scale bar: 5 μm. (e) Histogram representing the increase of FAPs number estimated from Vinculin staining in sh2 MCU cells compared to control. (mean ± S.E.M; 10 cells for each condition; n = 3 independent experiments). ***P < 0.001. (f) Histogram representing the increase of FAP size estimated from Vinculin staining in sh2 MCU cells compared to control cells. (mean ± S.E.M; 10 cells for each condition; n = 3 independent experiments). ***P < 0.001. (g) Immunoblot showing the effect of sh1 and sh2 MCU on phospho-Paxillin Y118 protein levels (P-Paxillin Y118). Quantitative ratios between P-Paxillin Y118 and total Paxillin are indicated below. Mcu knockdown leads to decreased P-Paxillin Y118/total Paxillin ratio. MCU antibody was used to show the efficiency of the shRNAs. F1F0 ATPase antibody was used as loading control. (h) Histogram presenting the decrease of Calpain activity measured in mcu-silenced cells and compared to control cells (mean ± S.E.M; n = 3 independent experiments). *P < 0.05, **P < 0.01. See also Supplementary Fig. S3.

MCU downregulation leads to reduced intracellular Ca2+ levels

Calpains are intracellular proteases, which require cytosolic Ca2+ ions for their activity44. We thus analyzed the basal cytosolic Ca2+ level in control versus mcu-silenced Hs578t cells, using the cytosolic Ca2+ dye Fluoforte. As shown in Fig. 4a, mcu silencing led to a significant decrease in the basal cytosolic Ca2+ pool (decrease of 13% and 17.1% for sh1 and sh2 MCU cells, respectively). These cytosolic and mitochondrial Ca2+ uptake reductions did not appear to correlate with a decrease in the mitochondrial bioenergetics. Indeed basal oxygen consumption rates (OCR) in mcu-silenced cells were found to be similar to control cells (Supplementary Fig. S4a,b). In the same line, we checked the global intracellular ATP levels in mcu-silenced and control cells. Actually, as shown in Fig. S4c, the global intracellular ATP levels were similar in mcu-silenced cells (6.22 μmol/g ± 0.1 and 7.65 μmol/g ± 0.25 for shRNA MCU #1 and #2, respectively), compared to controls (6.81 μmol/g ± 0.31). Together, these results indicate that the observed F-actin cytoskeleton phenotype is not due to a global intracellular ATP production default.

Figure 4: MCU knockdown results in intracellular Ca2+ impairment.
Figure 4

(a) Histogram showing the basal cytosolic Ca2+ levels ([Ca2+]i) of sh Control and sh1, sh2 MCU Hs578t cells using the cytosolic Ca2+ sensitive dye Fluoforte. Compared to control cells, mcu-silenced cells have lower basal cytosolic [Ca2+]i. Fluorescence intensities were reported as ratio to sh Control cells (mean ± S.E.M; n = 3 independent experiments; **P < 0.01, ***P < 0.001. (b) Representative trace of cytosolic Ca2+ rise following histamine (100 μM) stimulation using Fluoforte dye performed in control or mcu-silenced cells. Mcu-silencing led to a decrease in the ER-dependent cytosolic Ca2+ rise. Fluoforte fluorescence intensities were normalized to the baseline (F/F0 ratio). (c) Histogram depicting the maximum Ca2+-increase in the cytosol (Fmax/F0 ratio) in cells following histamine (100 μM) treatment, from (b). (mean ± S.E.M; n = 3 independent experiments). ***P < 0.001. (d) Representative trace of cytosolic Ca2+ rise following ER-Ca2+ leak induced by Thapsigargin (10 μM) stimulation. Mcu-silencing led to a decrease in the ER-dependent cytosolic Ca2+ rise. Fluoforte fluorescence intensities were normalized to the baseline (F/F0 ratio). (e) Histogram depicting the maximum Ca2+-release in the cytosol (Fmax/F0 ratio) in cells following thapsigargin (10 μM) treatment, from (d). (mean ± S.E.M; n = 3 independent experiments). ***P < 0.001. (f) Representative trace of the relative changes in the Fluoforte fluorescence intensities normalized to the baseline (F/F0 ratio). Following Thapsigargin (10 μM)-induced ER Ca2+ depletion, extracellular Ca2+ (2mM) was applied on the cells in order to measure SOCE efficiency corresponding to the maximum speed of Ca2+ influx. Mcu-silencing led to decrease SOCE efficiency compared to control cells. (g) Histogram depicting SOCE efficiency (speed max Ca2+ influx) measured in Hs578t cells stably expressing sh Control, sh1 MCU or sh2 MCU shRNAs, from (f) (mean ± S.E.M; n = 3 independent experiments) *P < 0.05; ***P < 0.001. See also Supplementary Fig. S4.

The decrease of basal intracellular Ca2+ levels in mcu-silenced cells suggested that intracellular compartments, including the ER, may have reduced Ca2+ buffering capacities. To test this hypothesis, we measured IP3-dependent ER Ca2+ release following histamine treatment. In control cells, histamine induces a rapid increase of cytosolic Ca2+ levels (2.4 fold; ± 0.09), in contrast to mcu-silenced cells (1.5 fold; ±0.03 for sh1 MCU; 1.8 fold; ±0.04 for sh2 MCU) (Fig. 4b,c).

The ER Ca2+ pool is directly dependent on the store operated Ca2+ entry (SOCE), which refills the ER lumen with Ca2+ ions from extracellular space45. This led us to analyze the passive ER Ca2+ leakage, by inhibiting the ER Ca2+ pump sarcoplasmic-endoplasmic reticulum Ca2+ ATPase (SERCA) with thapsigargin. In control cells, thapsigargin treatment induces a progressive increase of cytosolic Ca2+ levels, peaking at about 4 min post-incubation (Fluoforte Fmax/F0 ratio  = 2.79 ± 0.67) (Fig. 4d,e). In mcu-silenced cells, the ER Ca2+ leak was significantly decreased (Fluoforte Fmax/F0 ratio = 1.90 ± 0.21 and 1.87 ± 0.29 for si1 and si2 MCU, respectively) indicating a decrease of ER Ca2+ levels (Fig. 4d,e). Finally, we directly measured SOCE efficiency by inducing ER Ca2+ leakage by thapsigargin treatment in a Ca2+ free medium, followed by extracellular Ca2+ boost. As shown in Fig. 4f,g, in mcu-silenced cells, SOCE activity was strongly reduced (intracellular Ca2+ influx = 0.29 AU/s ± 0.04 AU/s for sh1 MCU; 0.48 AU/s ± 0.07 AU/s for sh2 MCU) compared to control cells (0.8 AU/s ± 0.1 AU/s). This was further confirmed using ionomycine to deplet the ER Ca2+ stores (Supplementary Fig. S4d,e). Altogether these results support the notion that the down regulation of the mitochondrial Ca2+ uptake in mcu-silenced cell, leads to a decrease of ER and cytosolic Ca2+ pools due to impairment of SOCE.

Cytosolic Ca2+ depletion phenocopies mcu knockdown phenotype

To confirm that direct SOCE impairment leads to cell migration and cytoskeleton defects similar to those observed following MCU silencing, we silenced STIM1 using three specific siRNAs (Supplementary Fig. S5a). In fact, all three siRNAs led to a significant decrease of cell migration (TTD of 160.70 μm ± 11.6 μm, 202.5 ± 16.6 μm, 185.50 μm ± 12.9 μm, compared to 383.7 μm ± 19.6 μm for si1–3 STIM1 and si Control, respectively) (Supplementary Fig. S5b,c) together with Vinculin accumulation in the FAPs (Supplementary Fig. S5d). These results show that the SOCE-dependent Ca2+ uptake sustains the migration capacities of Hs578t breast cancer cells.

To confirm the actual importance of cytosolic Ca2+, we treated Hs578t cells with the cell permeable Ca2+ chelator BAPTA-AM. Incubation with 5 μM of BAPTA-AM significantly decreased cell migration as measured by individual cell tracking over a period of 24 hours (Fig. 5a). Indeed, in BAPTA-AM treated cells the TTD was 178.8 μm ± 8.9 μm, compared to 299.4 μm ± 15.4 μm for control cells (Fig. 5b). Furthermore, BAPTA-AM treatment resulted in Vinculin accumulation in the FAPs at the periphery of the cells (Fig. 5c). Finally, we detected a significant decrease in Calpains activity in BAPTA-AM treated cells (Fig. 5d). Altogether these results show that the depletion of cytosolic Ca2+ phenocopies at the molecular level the silencing of mcu, highlighting the crucial role of mitochondrial Ca2+ uptake in cytoskeleton architecture and cell migration (Fig. 5e).

Figure 5: Pharmacological impairment of intracellular Ca2+ levels phenocopies mcu silencing.
Figure 5

(a) Representative cell paths (blue lines) of isolated Hs578t cells (red dots) treated with DMSO or the cell permeable Ca2+ chelator BAPTA-AM (5 μM); acquisition time 24 hours. BAPTA-AM led to decrease cell migration. (b) Histogram showing the decrease in the cell migration of BAPTA-AM treated cells (mean ± S.E.M; 30 cells in each experiment; n = 3 independent experiments). **P < 0.01. (c) Representative confocal images showing the accumulation of Vinculin in the FAPs in BAPTA-AM treated cells compared to DMSO treated controls. Vinculin and F-actin were stained using anti-Vinculin antibody and phalloidine rhodamine probe, respectively. Scale bar: 20 μm. (d) Histogram representing the Calpain activity measured in BAPTA-AM treated cells reported to control cells (mean ± S.E.M; n = 3 independent experiments). BAPTA-AM treatment led to a decrease Calpain activity. ***P < 0.001. (e) Schematic model showing the role of MCU in the control of Ca2+ homeostasis and cell migration. Mcu-silencing using si or shRNA strategies leads to SOCE impairment with subsequent decrease of the cytosolic Ca2+ levels ([Ca2+]c). This intracellular calcium reduction causes a decrease in the Rho family of GTPases and Calpains activities, which may alter the cytoskeleton dynamics and the migration of the cell. See also Supplementary Fig. S5.

Discussion

Cell migration is a highly dynamic process in which actin cytoskeleton remodeling and focal adhesion turnover orchestrate front-to-rear polarity and cell movements2. Lamellipodia formation at the front end is controlled by Rac1, whereas actomyosin contraction at the rear end is regulated by RhoA6. In addition, Calpains allow the degradation of FAPs, including Paxillin, which is required for proper rear end retraction7. In fact, a number of these events are Ca2+-dependent, further supporting that Ca2+ trafficking is critical for cell migration. We previously showed that alterations of mitochondrial Ca2+ buffering due to mcu silencing compromises the migration of the blastomeres in the developing zebrafish32. Here we show that in breast cancer and HeLa cells, mcu silencing leads to a strong inhibition of migration and loss of polarity. At the molecular level, this seems to be due to of F-actin fibers accumulation and FAPs stabilization. This phenotype appears to be mediated by the decrease of RhoA and Rac1 activities as well as downregulation of total Calpain activity, two Ca2+ dependent parameters. Actually, a direct lowering of intracellular Ca2+ levels using BAPTA-AM or inhibition of the SOCE by silencing STIM118 mimicked mcu knock down phenotype. Importantly, treatment of the cells with the potent MCU inhibitor Ru360, resulted in a decreased capacity of the cells to close the gap, which illustrates the primordial role of mitochondrial Ca2+ homeostasis in the cell migration process.

Interestingly, we also noticed a decrease of Paxillin phosphorylation on Y118, a known substrate of FAK, suggesting that this kinase might be down regulated in mcu-silenced cells. This hypothesis is further supported by the fact that FAK activity is regulated by the CaMKII and Calmodulin Ca2+-dependent pathways46,47. In addition, in these cells, the localization of FAK might also be altered since FAK association at FA48 and FAK/FAP interactions have been reported to depend on Ca2+49.

Given that FAK can also influence the activity of Rho-family GTPases50, it might be possible that the observed inhibition of small GTPases upon mcu silencing is due to the inhibition of FAK, thus shedding new light on the mechanisms that regulate cell migration via Ca2+ intracellular trafficking.

Cytosolic Ca2+ pulses are involved in cell directionality51 and lamellipodia retraction8. These microdomains, also called Ca2+ flickers are thought to be generated by Ca2+ entry from the plasma membrane51 and by IP3-induced Ca2+ release from the ER20. Here, we report that both cytosolic and ER Ca2+ pools are decreased in mcu knocked down cells, confirming the requirement of an intact mitochondrial Ca2+ uptake machinery to sustain SOCE18,38. In mcu-silenced cells, altered SOCE may thus compromise the generation of Ca2+ pulses, affecting in turn FAPs dynamics and cell migration. In fact, mcu silencing may impair the capacity of mitochondria to buffer Ca2+ flickers, particularly at the mitochondria/ER contact sites, where Ca2+ currents may take place52. Such mitochondrial impairment to buffer Ca2+ flickers may alter the physiological spatiotemporal Ca2+ distribution required for proper focal adhesion dynamics. This further supports the notion that the mitochondrial physiology has a role in cytoskeleton dynamics and cell migration. In this respect, we analyzed in Hs578t cells, the effect of mcu silencing on mitochondrial bioenergetics. Using Seahorse™ technology, we did not observe any significant difference in the OCR between control and mcu-silenced cells. Moreover, global intracellular ATP production measurement did not reveal any difference between mcu-silenced cells and controls suggesting that the observed cell migration phenotype is not due to an ATP production decrease, but is specific to the mitochondrial Ca2+ homeostasis deregulation.

Interestingly, it has been shown that mitochondria was involved in the ER- Ca2+ filling as well53. Indeed, in cardiac pacemaker cells under severe physiological stress, MCU is required for promoting oxidative phosphorylation and ATP production in a specific subcellular compartment required for the activity of SERCA2a and the reloading of ER Ca2+ stores54. Thus even if the global intracellular ATP production was not altered in mcu-silenced cells, we can not exclude that a site specific production of ATP at the mitochondria/ER contact points is specifically required for Actin cytoskeleton remodeling during cell migration.

Finally, our results, obtained in human cell lines, underscore the role of F-actin cytoskeleton dynamics as described in the nematode34 and the zebrafish32 models. Indeed, we previously showed that downregulation of MCU in zebrafish embryos led to a decrease in mitochondrial Ca2+ pool together with a dysregulation of F-actin protrusion dynamics, leading to major developmental defects32; however, the mechanism involved in actin dysregulation was not elucidated. An interesting study performed in C. elegans highlighted also the critical role of mitochondrial Ca2+ uptake in reactive oxygen species (ROS) production, which seems to be required for Actin cytoskeleton dynamics and wound healing34. Recently, MCU expression was linked to redox status in breast cancer cell lines. Indeed, downregulation of MCU was reported to decrease mitochondrial ROS production as well as hypoxia-inducible factor-1α expression, impacting cell migration and tumor progression37. However, in MDA-MB-213 breast carcinoma cells, manipulations of MCU and MICU1 have no effect on ROS production39. Further studies need to be performed to completely describe the potential connection between mitochondrial Ca2+ uptake, ROS generation and actin cytoskeleton dynamics.

Together, these present observations combined with previous studies reveal an additional mechanism by which mitochondrial Ca2+ uptake affects cytoskeleton dynamics and cell migration. Interestingly, it appears that the MCU contribution to cell migration is not restricted to cancer cells but rather reflects an evolutionary conserved process in eukaryotes, from worms to vertebrates.

Methods

Cell Lines

HeLa cervical cancer and Hs578t breast carcinoma cell lines, routinely checked for contaminations, were grown under standard cell culture conditions (37 °C, 5% CO2) in Dulbecco’s modified Eagle’s medium (DMEM) high glucose medium (Gibco) supplemented with 10% FBS (Sigma), 100 U/mL penicillin and 100 μg/mL streptomycin (Gibco).

RNA interference

Two siRNAs duplex targeting the 3′UTR sequence of mcu (NM_138357.1) were selected in the dataBase of Integrated DNA technologies (IDT). The first and second siRNAs, targeting the 3′UTR sequence of mcu (NM_138357.1), sense strands are:

Si1 MCU: 5′-GGAUCUCAAAGGGUGCAAUUUAUCT-3′.

Si2 MCU: 5′-GGAACCAACUUAUAACUGUUUAATA-3′.

The three siRNAs sequence of stim1 (NM_001277961.1) sense strands are:

Si1 STIM1 (targeting the CDS): 5′-GGUGCAAUAUUACAACAUCAAGAAG-3′

Si2 STIM1 (targeting the CDS): 5′-GAUGAGAUCAACCUUGCUAAGCAGG-3′

Si3 STIM1 (targeting the 3′UTR): 5′-GUUAUAAGGCAGUCACUUUUUCUCT-3′.

The Allstar negative control siRNA (Qiagen) was used as siRNA Control.

SiRNA transfection was performed using Lipofectamine RNAiMAX (Invitrogen) according to the manufacturer’s protocol. Cell analyses were performed 48 hours (h) post transfection.

Lentiviral infection

For mcu stable down-regulation, two Hs578t clones were generated by lentiviral infection with pSuperRetro vector containing MCU shRNA possessing the same two sequences of the Hairpin as the siRNA. ShRNA MCU expressing cells were selected using blasticidin (5 μg/mL). RhoA activity was detected using RhoA2G FRET based biosensor encoded by pLentiRhoA2G construction (Addgene #40179). Cells expressing RhoA2G were selected with puromycin (1 μg/mL).

Wound healing assays

Wound healing assays were performed in Hs578t cells. Briefly, 48 h post transfection cell layer at confluence was scratched in two orthogonal lines using sterile 10 μL pipette tip and washed two times with fresh medium. For Ru360 experiments (Calbiochem 557440), 4 × 105 cells were plated in 6-well plates and grown overnight. Ru360 (60 μM) was added in combination with Probenecib (Molecular Probes #P36400) at 2.5 mM to avoid cellular extrusion. Pictures were taken at 0 and 7.5 h post-wounding using inverted microscope (Zeiss). Cell free space was calculated using Image J software (NIH).

Boyden chamber migration assays

Boyden chamber migration assays were performed using FluoroBlok 96-multiwell insert plates (BD Falcon) with an 8 μm pore size PET membrane. Hs578t cells were cultured in serum-free medium 12 h prior to the cell migration assay. 1.25 × 105 cells were seeded in the upper chamber in serum-free medium; medium supplemented with 5% serum was used as a chemo-attractant in the lower chamber. The plates were incubated for 7.5 h; migrating cells were stained with 2 μM Calcein-AM Fluorescent Dye (Interchim). Cells were counted using a Zeiss inverted fluorescence microscope.

Cell tracking, proliferation and apoptosis detection

For cell tracking experiments, apoptosis and cell proliferation, Hs578t and HeLa cells were analyzed using IncuCyte live-content imaging system (Essen Bioscience). Briefly, cell tracking was performed on transfected cells seeded at 10% confluence in 24-well locked plates (Essen Bioscience). Images were automatically acquired every 30 minutes (min) for 48 h at 4X magnification (single images). Cells were tracked for 24 h; cell coordinates were acquired using ImageJ software. The total distance was calculated with Excel house made algorithm (Microsoft). Apoptosis was detected using Caspase-3/7 apoptosis assay reagent at 2.5 μM concentration (Essen Bioscience #4440). Images were automatically acquired in phase and green fluorescence channels every 30 min for 48 h at 4X magnification. Data were proceeded using a dedicated algorithm (Essen Bioscience). Cell proliferation was estimated using the phase-contrast images of the same experiments.

Live cell imaging

Videomicroscopy experiments were performed on Hs578t, stably expressing shcontrol or sh-MCU RNAs. Cells were monitored every minute for 5 h. Pictures were taken at 20X magnification using a Zeiss Axiovert 200 microscope.

Paxillin dynamics were analyzed using Hs578t cells transiently transfected with pEGFP-Paxillin. Twenty-four h after transfection cells were seeded at 10% confluence in 8 well Nunc™ Lab-Tek™ II Chamber Slide (Thermo Scientific). Images at 60X magnification were acquired every min for 20 min for Paxillin-GFP using a Zeiss 780 confocal microscope equipped with chamber preheated at 37 °C in presence of 5% CO2.

RhoA activation

RhoA activity was analyzed using Hs578t cells stably expressing RhoA2G biosensor. Twenty-four h before measurements cells were seeded at 10% confluence in 8 well Nunc™ Lab-Tek™ II Chamber Slide (Thermo Scientific). Images were acquired on isolated cells expressing low levels of the RhoA2G as previously described40 with the following modifications. Fluorescence excitation was performed using 405 nm laser and detection filters were set at 480/40 nm (donor channel) and 535/30 nm (FRET channel) using a Zeiss 780 confocal microscope. Images were acquired every second (sec) for 4 min. After 15 sec of basal recoding, histamine (100 μM final concentration) was added to the cells. For RhoA2G positive control, cells were treated with Thrombin 1 U/μL. FRET to donor channel ratio at the cell protusion area of individual cell was calculated using image J software.

Oxygen Consumption Rate (OCR) and ATP measurements

OCRs were measured using a Seahorse Bioscience XF24 Extracellular Flux Analyzer (Seahorse Bioscience, North Billerica, MA) according to the manufacturer’s protocol. Cells were seeded in normal growth medium 24 h before measurement at a density of 5 × 104 cells per well for Hs578t sh Control, sh1 MCU and sh2 MCU cells. The assay was performed in XF minimal basal medium (Seahorse Bioscience) supplemented with 25 mM glucose, 1 mM sodium pyruvate, 4 mM glutamine, 10% FBS at pH 7.4. Cells were pre-incubated in this medium for 1 h before measurement at 37 °C in a humidified atmosphere without CO2. Oligomycin A (0.5 μM), FCCP (1 μM), rotenone (0.5 μM), antimycin A (0.5 μM) were used to evaluate mitochondrial respiratory capacity. The data were normalized by the amount of protein present in each well.

Intracellular ATP levels in Hs578t cells expressing sh Control and the two sh MCU RNAs were assessed using ATP Assay Kit (Abcam) following manufacturer’s instructions. Clariostar microplate fluorescence reader (BMG Labtech) was used for the measure of fluorescence (Ex/Em = 535/587 nm).

BAPTA-AM treatment

BAPTA-AM treatment was performed by incubation of Hs578t cells with 5 μM of BAPTA-AM (Enzo BML CA 411 0025) for 1 h at 37 °C, followed by Calpains activity measurements or immunofluorescence analyses. Cells were tracked for 24 h.

Ca2+ measurements

Cytosolic Ca2+ levels were detected in HeLa and Hs578t cells using Fluoforte dye (Enzo Life Sciences). Cells seeded in 96-well plates were incubated with 5 μM Fluoforte for 1 h at 37 °C, in a Ca2+-free balanced salt solution (BSS) [121 mM NaCl, 5.4 mM KCl, 0.8 mM MgCl2, 6 mM NaHCO3, 5.5 mM D-Glucose, 25 mM Hepes (pH 7.3)]. Raw fluorescence values were collected every 0.21 sec for 2 min at 28 °C using Clariostar microplate fluorescence reader (BMG Labtech). After 5 sec of basal line measurement, 100 μM histamine (Sigma) was injected.

For basal Ca2+ measurements the Fluoforte fluorescence signals were normalized to total protein levels using Bradford assay.

For ER-Ca2+ leakage experiments Fluoforte loaded HeLa cells, transfected with control,or MCU siRNAs, were treated with 10 μM thapsigargin (Enzo Life Sciences) as described previously55. Fluorescence signals were recorded using Zeiss 780 confocal microscope. Fluorescence excitation was performed using 488 nm laser and detection filters were set at 533/40 nm using a Zeiss 780 confocal microscope. Images were acquired every sec for 2 min.

SOCE measurements were performed on Hs578t cells expressing sh Control and the two sh-MCU RNAs. Cells were incubated during 1 h with 5 μM Fluoforte dye, and washed with BBS containing 0.1 mM EGTA. After 20 sec of baseline, Thapsigargin 10 μM was added, and 5 min later 2 mM of CaCl2 was added.

Mitochondrial Ca2+ measurements on siRNA transfected or shRNA expressing Hs578t cells were performed using Rhod-2 AM chemical dye or CEPIA2mt recombinant protein, respectively. Rhod-2 detection was performed as previously described for Fluoforte with the following modifications. Rhod-2 AM dye was incubated at 2.5 μM with 0.2% of pluronic acid (Molecular probes) for 20 min at 37 °C in BBS-Ca2+ (BBS supplemented with 2 mM of Ca2+), and washed for 20 min with BBS-Ca2+at room temperature. Raw fluorescence values were collected every 0.21 sec for 2 min at room temperature using Clariostar microplate fluorescence reader.

For CEPIA2mt detection, Hs578t expressing sh Control or the two sh-MCU RNAs were transfected with pCMV CEPIA2mt (Addgene #58218) and seeded at 40% in 8 well Nunc™ Lab-Tek™ II Chamber Slide. Twenty-four h later, cells were washed with BBS-Ca2+. After 10 sec of baseline, 100 μM of histamine was added. Fluorescence excitation was performed using 488 nm laser and detection filters were set at 533/40 nm using a Zeiss 780 confocal microscope. Images were acquired every sec for 5 min.

Mitochondrial Ca2+ uptake on isolated mitochondria was performed as previously described32 with the following modifications. Hs578t cells were transfected with si1 and si2 MCU siRNAs as well as control siRNA. Forty eight h later, two 10 cm petri dishes were washed 2 times with PBS and cells were scraped with 1 mL ice cold MB buffer (210 mM mannitol, 70 mM sucrose, 1 mM EDTA, 10 mM HEPES [pH 7.5] containing proteases inhibitors). Ca2+ measurements were perfomed using Clariostar microplate fluorescence reader (Ex/Em = 492/517 nm).

ER Ca2+ filling capacities in Hs578t expressing sh Control and the two sh-MCU RNAs were measured using the ER probe R-CEPIA1er recombinant protein. Cells were transfected with pCMV R-CEPIA1er (Addgene #58216). Cells were seeded at 40% confluence in 8 well Nunc™ Lab-Tek™ II Chamber Slide. Twenty four h later cells were washed with BBS-Ca2+ and incubated with ionomycin (10 μM). Fluorescence excitation was performed using 488 nm laser and detection filters were set at 533/40 nm using a Zeiss 780 confocal microscope. Images were acquired every sec for 5 min.

Detection of Calpains activity and activated Rac1

Calpains activity was measured in MCU and control shRNAs Hs578t cell lines using a Calpains Activity Assay Kit (Abcam #ab65308) following manufacturer’s instructions. Briefly, for every measurement, 1.5 × 106 cells of each condition were lysed with extraction buffer and fluorescence was evaluated using excitation filter: 400 nm ± 15 nm and emission filter: 505 nm ± 15. Activated Rac1 form was detected using RhoA/Rac1/Cdc42 Activation Assay Combo Kit (Cell Biolabs) following the manufacturer’s instructions.

Western blot analyses and antibodies

Western blots were performed as previously described56. The following antibodies were used: MCU (Abcam #Ab121499; dilution: 1/500), F1F0 ATPase (BD #612518; dilution: 1/1000), Vinculin (Santa Cruz #sc-55465; dilution: 1/2000), Paxillin H114 (Santa Cruz #sc-5574; dilution: 1/1000), Phospho-Paxillin Tyr 118 (Cell Signaling Technology #2541; dilution: 1/1000), Phospho-Myosin light chain 2 (Cell Signaling Technology #3671; dilution: 1/1000), STIM1 (Abcam #Ab57834; dilution: 1/1000) and Rac1 (Cell Biolabs #240106; dilution: 1/1000).

Immunofluorescence

Hs578t cells were seeded on a glass coverslip in 6-well plates at 50% of confluence. Following cell attachment the medium was removed and cell were fixed with 4% Paraformaldehyde containing 0.3% Triton X100. Cells were washed three times in 1X PBS and incubated with blocking buffer (0.1% Triton X100, 3% BSA in PBS). Vinculin antibody (Sigma #V4505; dilutiom: 1/50) was used to detect the FAPs. Phospho-Myosin light chain-2 antibody (Cell Signaling Technology #3671) was used at 1/50 dilution. F-Actin was stained with rhodamine phalloidin dye (Invitrogen #R415) at 1/200 dilution. Nuclei were visualized using Hoecht 33342 dye (Invitrogen #H3570) at 10 μg/mL. Images were acquired under a Zeiss 780 confocal microscope.

Statistical analyses

Error bars displayed on graphs represent standard errors of the mean (S.E.M) of at least three independent experiments. Statistical significance was determined using the unpaired two-sample Student’s T-test with the following convention: *P < 0.05, **P < 0.01, ***P < 0.001.

Additional Information

How to cite this article: Prudent, J. et al. Mitochondrial Ca2+ uptake controls actin cytoskeleton dynamics during cell migration. Sci. Rep. 6, 36570; doi: 10.1038/srep36570 (2016).

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References

  1. 1.

    & Tumour-cell invasion and migration: diversity and escape mechanisms. Nat. Rev. Cancer 3, 362–374 (2003).

  2. 2.

    , & Cell adhesion: integrating cytoskeletal dynamics and cellular tension. Nat. Rev. Mol. Cell Biol. 11, 633–643 (2010).

  3. 3.

    , , & Mechanical integration of actin and adhesion dynamics in cell migration. Annu. Rev. Cell Dev. Biol. 26, 315–333 (2010).

  4. 4.

    , & Focal adhesion kinase: in command and control of cell motility. Nat. Rev. Mol. Cell Biol. 6, 56–68 (2005).

  5. 5.

    et al. Lamellipodial Actin Mechanically Links Myosin Activity with Adhesion-Site Formation. Cell 128, 561–575 (2007).

  6. 6.

    et al. Coordination of Rho GTPase activities during cell protrusion. Nature 461, 99–103 (2009).

  7. 7.

    , , & Degraded Collagen Fragments Promote Rapid Disassembly of Smooth Muscle Focal Adhesions That Correlates with Cleavage of pp125FAK, Paxillin, and Talin. J. Cell Biol. 147, 619–629 (1999).

  8. 8.

    & Ca2+ pulses control local cycles of lamellipodia retraction and adhesion along the front of migrating cells. Curr. Biol. 22, 837–842 (2012).

  9. 9.

    et al. Periodic lamellipodial contractions correlate with rearward actin waves. Cell 116, 431–443 (2004).

  10. 10.

    et al. A role for actin arcs in the leading-edge advance of migrating cells. Nat. Cell Biol. 13, 371–381 (2011).

  11. 11.

    , , & Regulation of focal complex composition and disassembly by the calcium-dependent protease calpain. J. Cell Sci. 115, 3415–3425 (2002).

  12. 12.

    et al. Calpain-mediated proteolysis of talin regulates adhesion dynamics. Nat. Cell Biol. 6, 977–983 (2004).

  13. 13.

    , , & Mitochondria as sensors and regulators of calcium signalling. Nat. Rev. Mol. Cell Biol. 13, 566–578 (2012).

  14. 14.

    , , & Microdomains with high Ca2+ close to IP3-sensitive channels that are sensed by neighboring mitochondria. Science . 262, 744–747 (1993).

  15. 15.

    , & Regulation of plasma membrane calcium fluxes by mitochondria. Biochim Biophys Acta 1787, 1383–1394 (2009).

  16. 16.

    , & Store-operated Ca2+ entry depends on mitochondrial Ca2+ uptake. EMBO J . 21 (2002).

  17. 17.

    et al. Mitochondrial Ca2+ uptake and not mitochondrial motility is required for STIM1-Orai1-dependent store-operated Ca2+ entry. J. Cell Sci. 123, 2553–2564 (2010).

  18. 18.

    et al. IP3-mediated STIM1 oligomerization requires intact mitochondrial Ca2+ uptake. J. Cell Sci. 127, 2944–2955 (2014).

  19. 19.

    et al. The ER Ca2+ sensor STIM1 regulates actomyosin contractility of migratory cells. J. Cell Sci. 126, 1260–1267 (2013).

  20. 20.

    et al. A polarized Ca2+, diacylglycerol and STIM1 signalling system regulates directed cell migration. Nat. Cell Biol. 16, (2014).

  21. 21.

    , & Orai1 and STIM1 Are Critical for Breast Tumor Cell Migration and Metastasis. Cancer Cell 15, 124–134 (2009).

  22. 22.

    et al. Integrative genomics identifies MCU as an essential component of the mitochondrial calcium uniporter. Nature 476, 341–345 (2011).

  23. 23.

    , , , & A forty-kilodalton protein of the inner membrane is the mitochondrial calcium uniporter. Nature 476, 336–340 (2011).

  24. 24.

    et al. MICU1 encodes a mitochondrial EF hand protein required for Ca(2+) uptake. Nature 467, 291–296 (2010).

  25. 25.

    et al. MICU2, a Paralog of MICU1, Resides within the Mitochondrial Uniporter Complex to Regulate Calcium Handling. PLoS One 8, e55785 (2013).

  26. 26.

    et al. EMRE is an essential component of the mitochondrial calcium uniporter complex. Science 342, 1379–1382 (2013).

  27. 27.

    et al. The physiological role of mitochondrial calcium revealed by mice lacking the mitochondrial calcium uniporter. Nat. Cell Biol. 15, 1464–1472 (2013).

  28. 28.

    et al. The Mitochondrial Calcium Uniporter Controls Skeletal Muscle Trophism In Vivo Report The Mitochondrial Calcium Uniporter Controls Skeletal Muscle Trophism In Vivo. CellReports 10, 1269–1279 (2015).

  29. 29.

    et al. The Mitochondrial Calcium Uniporter Matches Energetic Supply with Cardiac Workload during Stress and Modulates Permeability Transition. Cell Rep . 1–12, doi: 10.1016/j.celrep.2015.06.017 (2015).

  30. 30.

    et al. The Mitochondrial Calcium Uniporter Selectively Matches Metabolic Output to Acute Contractile Stress in the Heart. Cell Rep . 1–8, doi: 10.1016/j.celrep.2015.06.002 (2015).

  31. 31.

    et al. Inhibition of MCU forces extramitochondrial adaptations governing physiological and pathological stress responses in heart. Proc Natl Acad Sci USA. 112, 9129–34. doi: 10.1073/pnas.1504705112 (2015).

  32. 32.

    et al. Bcl-wav and the mitochondrial calcium uniporter drive gastrula morphogenesis in zebrafish. Nat. Commun. 4, 2330 (2013).

  33. 33.

    , & Essential regulation of cell bioenergetics in Trypanosoma brucei by the mitochondrial calcium uniporter. Nat. Commun. 4, 2865 (2013).

  34. 34.

    & C. elegans Epidermal Wounding Induces a Mitochondrial ROS Burst that Promotes Wound Repair. Dev. Cell 31, 48–60 (2014).

  35. 35.

    & The mitochondrial calcium uniporter complex: molecular components, structure and physiopathological implications. J. Physiol. 0, 1–11 (2013).

  36. 36.

    et al. MICU1 motifs define mitochondrial calcium uniporter binding and activity. Cell Rep . 5, 1576–1588 (2013).

  37. 37.

    et al. The mitochondrial calcium uniporter regulates breast cancer progression via HIF-1. EMBO Mol. Med. 8, 569–585 (2016).

  38. 38.

    et al. Mitochondrial Ca(2+) uniporter is critical for store-operated Ca(2+) entry-dependent breast cancer cell migration. Biochem. Biophys. Res. Commun. 458, 186–193 (2015).

  39. 39.

    , , , & Mitochondrial Calcium Uniporter Activity Is Dispensable for MDA-MB-231 Breast Carcinoma Cell Survival. PLoS One 9, e96866 (2014).

  40. 40.

    et al. A versatile toolkit to produce sensitive FRET biosensors to visualize signaling in time and space. Sci. Signal. 6, rs12 (2013).

  41. 41.

    et al. Activation of RhoA by Thrombin in. Circ. Res. 335–340, doi: 10.1161/01.RES.87.4.335 (2000).

  42. 42.

    & Regulation of actin assembly associated with protrusion and adhesion in cell migration. Physiol. Rev. 88, 489–513 (2008).

  43. 43.

    , , & A paxillin tyrosine phosphorylation switch regulates the assembly and form of cell-matrix adhesions. J. Cell Sci. 120, 137–148 (2007).

  44. 44.

    , , , & The calpain system. Physiol Rev 83, 731–801 (2003).

  45. 45.

    , , & STIM proteins: dynamic calcium signal transducers. Nat. Rev. Mol. Cell Biol. 13, 549–565 (2012).

  46. 46.

    , , , & G protein-coupled receptor activation rapidly stimulates focal adhesion kinase phosphorylation at Ser-843: Mediation by Ca2+, calmodulin, and Ca2+/calmodulin-dependent kinase II. J. Biol. Chem. 280, 24212–24220 (2005).

  47. 47.

    , , & CaMK-II promotes focal adhesion turnover and cell motility by inducing tyrosine dephosphorylation of FAK and paxillin. Cell Motil. Cytoskeleton 65, 662–674 (2008).

  48. 48.

    et al. Calcium rises locally trigger focal adhesion disassembly and enhance residency of focal adhesion kinase at focal adhesions. J. Biol. Chem. 279, 28715–28723 (2004).

  49. 49.

    et al. ORAI1 calcium channel orchestrates skin homeostasis. Proc. Natl. Acad. Sci. USA 110, E4839–E4848 (2013).

  50. 50.

    et al. Focal adhesion kinase suppresses Rho activity to promote focal adhesion turnover. J. Cell Sci. 113 (Pt 2) 3673–3678 (2000).

  51. 51.

    et al. Calcium flickers steer cell migration. Nature 457, 901–905 (2009).

  52. 52.

    et al. Imaging interorganelle contacts and local calcium dynamics at the ER-mitochondrial interface. Mol. Cell 39, 121–132 (2010).

  53. 53.

    , , & The role of mitochondria for Ca2+ refilling of the endoplasmic reticulum. J. Biol. Chem. 280, 12114–12122 (2005).

  54. 54.

    et al. The mitochondrial uniporter controls fight or flight heart rate increases. Nat. Commun. 6, 6081 (2015).

  55. 55.

    et al. MAPL SUMOylation of Drp1 Stabilizes an ER/Mitochondrial Platform Required for Cell Death. Mol. Cell 59, 941–955 (2015).

  56. 56.

    et al. The Apoptotic Regulator Nrz Controls Cytoskeletal Dynamics via the Regulation of Ca(2+) Trafficking in the Zebrafish Blastula. Dev Cell 20, 663–676 (2011).

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Acknowledgements

We would like to thanks Dr Ivan Mikaelian for pEGFP-Paxillin and pLentiRhoA2G vectors. This work was supported by Ligue nationale contre le cancer (comité de la Drôme et du Rhône), Fondation ARC pour la recherche sur le cancer, AFM and the Medical Ressearch Council. MD is supported by a la ligue nationale contre le cancer fellowship.

Author information

Author notes

    • Julien Prudent
    • , Nikolay Popgeorgiev
    •  & Rudy Gadet

    These authors contributed equally to this work.

Affiliations

  1. Medical Research Council, Mitochondrial Biology Unit, Cambridge Biomedical Campus, Hills Road, Cambridge CB2 0XY, UK

    • Julien Prudent
  2. Université de Lyon, Centre de recherche en cancérologie de Lyon, U1052 INSERM, UMR CNRS 5286, Université Lyon I, Centre Léon Bérard, 28 rue Laennec, 69008 Lyon, France

    • Nikolay Popgeorgiev
    • , Rudy Gadet
    • , Mathieu Deygas
    • , Ruth Rimokh
    •  & Germain Gillet
  3. Hospices civils de Lyon, Laboratoire d’anatomie et cytologie pathologiques, Centre Hospitalier Lyon Sud, Chemin du Grand Revoyet, 69495 Pierre Bénite, France

    • Germain Gillet

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Contributions

J.P., N.P., R.R. and G.G. designed the experiments; N.P., R.G. and M.G. performed the experiments; J.P. and N.P. analyzed the results; J.P. initiated the project; J.P., N.P. and G.G. wrote the manuscript.

Competing interests

The authors declare no competing financial interests.

Corresponding authors

Correspondence to Julien Prudent or Nikolay Popgeorgiev.

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