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. 2011 May 17;22(1):127–141. doi: 10.1038/cr.2011.82

Caspase cleavage of cytochrome c1 disrupts mitochondrial function and enhances cytochrome c release

Yushan Zhu 1,2,*, Min Li 3,*, Xiaohui Wang 1, Haijing Jin 1, Shusen Liu 1, Jianxin Xu 3,*, Quan Chen 1,2,*
PMCID: PMC3351920  PMID: 21577235

Abstract

Mitochondrial catastrophe can be the cause or consequence of apoptosis and is associated with a number of pathophysiological conditions. The exact relationship between mitochondrial catastrophe and caspase activation is not completely understood. Here we addressed the underlying mechanism, explaining how activated caspase could feedback to attack mitochondria to amplify further cytochrome c (cyto.c) release. We discovered that cytochrome c1 (cyto.c1) in the bc1 complex of the mitochondrial respiration chain was a novel substrate of caspase 3 (casp.3). We found that cyto.c1 was cleaved at the site of D106, which is critical for binding with cyto.c, following apoptotic stresses or targeted expression of casp.3 into the mitochondrial intermembrane space. We demonstrated that this cleavage was closely linked with further cyto.c release and mitochondrial catastrophe. These mitochondrial events could be effectively blocked by expressing non-cleavable cyto.c1 (D106A) or by caspase inhibitor z-VAD-fmk. Our results demonstrate that the cleavage of cyto.c1 represents a critical step for the feedback amplification of cyto.c release by caspases and subsequent mitochondrial catastrophe.

Keywords: cytochrome c1 cleavage, mitochondrial catastrophe, caspase, apoptosis

Introduction

Mitochondria are the intracellular powerhouse where energy substrates are metabolized to fuel the oxidative respiration reaction through the energy-transducing electron transport chain in the mitochondrial inner membrane. The oxidative respiratory chain consists of four multimeric complexes, which transfer electrons from the reducing substrates to oxygen to build up a proton gradient for adenosine-triphosphate (ATP) generation 1, 2, 3. The cytochrome bc1 complex is the central component of the oxidative respiratory reaction chain that oxidizes ubiquinol and reduces cytochrome c (cyto.c). The interaction between cytochrome c1 (cyto.c1) and cyto.c ensures the fast complex formation, optimal orientation and distance for electron transfer and also fast dissociation after electron transfer, which is critical for maintaining the electron flow and preventing the potential electron leak 4, 5. The cytochrome bc1 complex is also the major pathway for free radical generation within mitochondria 6, 7, 8. Disruption of this interaction results in the loss of the oxidative phosphorylation, ample generation of reactive oxygen species (ROS) and disruption of mitochondrial functions and physiology leading to cell death. These mitochondrial metabolic catastrophes are causally associated with apoptosis at the cellular level and diseases in the pathophysiological conditions 9, 10, 11.

Mitochondrial catastrophe could be both the cause and consequence of apoptosis. Mitochondria sense the metabolic catastrophic signals and commit cells to apoptosis by releasing death-inducing factors such as cyto.c into the cytosol due to the permeabilization of mitochondrial outer membrane 12, 13. The release of cyto.c could result in mitochondrial respiration failure and the loss of mitochondrial functions. Once released into the cytosol, cyto.c binds to apoptotic protease-activating factor 1 (Apaf-1) to form a complex termed the apoptosome 14, 15, 16, 17, which in turn leads to the activation of downstream caspases and subsequent cleavage of cellular substrates at a specific tetra-peptide sequence on the carboxyl side of aspartate residues. Interestingly, it has been shown that mitochondrial catastrophes, including the loss of mitochondrial membrane potential following cyto.c release and the burst of ROS production, depend on the caspase activation in some systems 18, 19, 20, 21, 22. Both pro- and activated caspases have been found in the mitochondrial intermembrane space 23, 24, 25, where they may disrupt mitochondrial function at the site of complex I and II 26, 27. We previously showed that there were two distinct stages of cyto.c release into the cytosol during apoptosis and the activated caspases could cause further cyto.c release 4, 28, 29. However, the molecular targets of caspase 3 (casp.3) and the precise mechanism of the amplification of cyto.c release by caspases are poorly understood. Here we report that cyto.c1 in the bc1 complex could be a novel target of casp.3 both in vitro and in cells. This cleavage of cyto.c1 is critical for the amplification of cyto.c release and mitochondrial dysfunction. Our results are the first to show that the cleavage of cyto.c1, a key partner for cyto.c, results in further amplification of cyto.c release and subsequent mitochondrial catastrophe.

Results

Recombinant casp.3 inhibits mitochondrial respiratory activity

We previously observed that activated casp.3 can induce cyto.c release, a rapid increase of ROS and the loss of integrity of isolated mitochondria 4. We here specifically determined if recombinant human casp.3 could disrupt the mitochondrial respiratory chain responsible for electron transfer and the mitochondrial ROS production. We first examined the effects of casp.3 on the succinate-cyto.c reductase (SCR) and cyto.c oxidase activity. Mitochondria isolated from mouse liver were incubated with or without casp.3 at 37 °C for various times, the activities of SCR and cyto.c oxidase were measured by the reduction or oxidation rate of exogenous cyto.c, respectively. Our result showed that recombinant casp.3 significantly inhibited the SCR activity in a time-dependent manner (Figure 1A) and strongly induced the spontaneous generation of ROS in mitochondria in the presence of succinate (Figure 1B). The H2O2 generation from mitochondria was measured using the method of luminol as previously described. This event could be inhibited by z-VAD-fmk, a pan caspase inhibitor (Figure 1B). Although recombinant casp.3 has no effect on the activity of complex IV (Figure 1C), it potently inhibits the activity of complex III as measured by reduction of oxidized cyto.c (Figure 1D). Taken together, we conclude that complex III could be specifically targeted by recombinant casp.3.

Figure 1.

Figure 1

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Recombinant casp.3 disrupts mitochondrial functions and physiology in vitro. (A) The activity of SCR was decreased by casp.3 treatment in a time-dependent manner. SCR from mouse liver was incubated with or without recombinant casp.3 at 37 °C for the indicated times. The SCR activities were then measured by the reduction rate of cyto.c. (B) The effects of activated recombinant casp.3 on mitochondrial ROS generation. Mitochondria extracted from mouse liver were incubated with different dosage of casp.3 at 37 °C for 1 h and the mitochondrial ROS generation was detected by LDCL. Antimycin A was used as a positive control. (C) The activated recombinant casp.3 has no effect on the complex IV activity. Mitochondria extracted from mouse liver were incubated with or without casp.3 at 37 °C for the indicated times and the complex IV activity was detected by the oxidation of endogenous cyto.c. (D) The activated recombinant casp.3 reduces the complex III activity. Mitochondria extracted from mouse liver were incubated with or without casp.3 at 37 °C for the indicated times and by using reduced quinine as the substrate, the complex III activity was demonstrated by the reduction of endogenous cyto.c. The data were the representative or mean value of at least 3 separate experiments.

Identification of cyto.c1 as a casp.3 substrate

In order to identify the potential substrate of casp.3 in the complex III, we purified SCR from pig hearts, in which the enzyme is highly conserved 30. The complex III was treated with recombinant casp.3 and Coomassie blue-stained diagonal gels were used to resolve the cleavage product, followed by SDS-PAGE analysis in the second dimension 18, 26. The two spots with a molecular size of about 10 and 25 kD as indicated in Figure 2A were further analyzed by MALDI-TOF-MS. Both were identified as cyto.c1, a key partner of cyto.c for the electron transfer in the mitochondrial respiratory chain and a highly conserved protein from yeast to human. To confirm that cyto.c1 is indeed a substrate of casp.3, the mouse liver mitochondria were incubated with recombinant casp.3 and the cleaved products were determined by western blotting analysis (Figure 2B). We next examined if endogenous cyto.c1 cleavage occurs in HeLa cells undergoing apoptosis. Cyto.c1 was found to be cleaved at 6 h after casp.3 was activated at 3 h in the cells treated with staurosporine (STS) (Figure 2B). The casp.3-deficient mouse embryonic fibroblast (MEF) also demonstrated that casp.3 is responsible for the cleavage of endogenous cyto.c1 and decreased apoptosis (Supplementary information, Figure S1).

Figure 2.

Figure 2

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Identification of cyto.c1 as a novel casp.3 substrate. (A) Coomassie-stained diagonal gels analysis reveals that a component of SCR is cleaved by recombinant casp.3. SCR from swine heart were resolved by SDS-PAGE, and the lane was rehydrated in the presence of recombinant casp.3 and resolved by SDS-PAGE in the second dimension. The two arrows indicate the spots corresponding to cyto.c1 as determined by MALDI-TOF-MS. (B) Cyto.c1 as a novel casp.3 substrate. Upper panel: mitochondria extracted from mouse liver were incubated with casp.3 at 37 °C for the indicated times in the presence or absence of z-VAD-fmk. Cyto.c1 cleavage was assessed by western blotting analysis. Lower panel: HeLa cells were treated with STS and the cell lystes were subjected to western blotting with anti-cyto.c1 or anti-casp.3 antibody. (C) Sequence alignment of the evolutionally conserved amino acids of cyto.c1 from several species. Residues that are identical and similar among the cyto.c1 are denoted in yellow and blue, respectively. The mutation sites are indicated by arrows. (D) Identification of D106 as a cleavage site. A volume of 20 μg of isolated mitochondria from wt cyto.c1, D106A, D128A and D157A cells were treated with 200 ng of activated recombinant casp.3 at 37 °C for 2 h in 50 μl of reaction buffer in vitro. The reactions were stopped and resolved by 15% SDS-PAGE and subjected to western blotting with anti-myc antibody.

As shown in Figure 2B, casp.3 was able to cleave cyto.c1 at the C-terminus to produce a peptide around 25 kD and this cleavage could be completely inhibited by z-VAD-fmk. Based on the sequence analysis (Figure 2C), several highly conserved Asp amino acid residues in cyto.c1 were mutated to Ala and the caspase cleavage analysis revealed that only the mutant with Asp mutation at residue 106, not at residues 128 and 157, was resistant to casp.3 cleavage under the same experimental conditions (Figure 2D), suggesting that D106 is the specific cleavage site of casp.3. Although it is not a typical casp.3 cleavage site, it is interesting to note that this site is exposed to the intermembrane space and close to the heme and cyto.c-binding sites 34. These data implicates that the cleavage of cyto.c1 by casp.3 may occur in the intermembrane space and could have a profound impact on mitochondrial functions and apoptosis.

Conversion of D106 to A in human cyto.c1 prevents STS-induced apoptosis and cyto.c release

In light of the importance of the interaction of cyto.c1 with cyto.c for the electron transfer and ROS generation, we determined the consequence of cyto.c1 cleavage in mitochondrial functions and apoptosis. Cells expressing wt (wild type) and non-cleavable form (D106 to A) human cyto.c1 were selected by Zeocin. As shown in Figure 3A and 3B, the cells expressing the non-cleavable form of cyto.c1 were clearly resistant to STS-induced apoptosis. Both casp.3 activation and cyto.c release were observed between 3-6 h after STS treatment as monitored by immunoblotting analysis (Figure 3B and 3C) and time lapse imaging of activated caspases (Supplementary information, Data S1, Figure S2 and Video S1A). Importantly, these events could be completely inhibited in the non-cleavable cyto.c1 or z-VAD-fmk. (Figure 3A-3C and Supplementary information, Figure S2, Video S1B and S1C).

Figure 3.

Figure 3

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Non-cleavable cyto.c1 abrogates STS-induced apoptosis and cyto.c release. (A) Non-cleavable cyto.c1 prevents STS-induced apoptosis. Left: flow cytometric analysis of apoptosis in cells expressing different mutant cyto.c1 following treatment with STS for 24 h. The percentage of Annexin V/PI positive cells was determined. Right: flow cytometric analysis of apoptosis in cells expressing wt and non-cleavable cyto.c1 exposed to STS (0.1 μM) for the indicated times. (B) Non-cleavable cyto.c1 prevents cyto.c release. Left: cells expressing wt or non-cleavable cyto.c1 were exposed to STS for the indicated times and subjected to subcellular fractionation. The cytosolic fraction (Cytosol) and mitochondrial fraction (Mito.) were analyzed by immunoblotting with anti-cyto.c antibody. Right: immunofluorescent microscopy of cyto.c release in wt and non-cleavable cyto.c1 cells treated with STS for 24 h. (C) Non-cleavable cyto.c1 blocks casp.3 activation and PARP cleavage. Cells expressing wt or non-cleavable cyto.c1 were treated with STS for the indicated times, followed by immuoblotting analysis with anti-casp.3 (upper) or anti-PARP antibodies (lower). (D) The effect of exogenous wt and non-cleavable cyto.c1 on cell death in cyto.c1 shRNA cells. The wt or non-cleavable mouse cyto.c1 was reintroduced into the endogenous cyto.c1-knockdown HeLa cells and the protein level of cyto.c1 was detected (upper). Lower panel showed flow cytometric analysis of apoptosis exposed to STS. The data were the representative or mean value of at least three separate experiments and statistical significance was determined by Student's t-test, *P < 0.05.

As cyto.c1 is an important partner of cyto.c for mitochondrial respiration, its cleavage could strikingly affect the release of cyto.c from mitochondria, leading to the amplification of apoptotic cascade. To address this possibility, the release of cyto.c was detected by both immunofluorescence and cell fractionation methods. Our results showed that cyto.c was released from mitochondria starting at 3 h in the cells expressing wt cyto.c1. In contrast, the cyto.c release was completely abrogated in the cells expressing the non-cleavable form of cyto.c1 (Figure 3B). To further substantiate this observation, we took an approach to transfect GFP-tagged cyto.c into HeLa cells and monitored the cyto.c release following the treatment of death stimuli. Clearly, we showed that the cyto.c release from mitochondria become visible at about 5 h after the exposure of STS in wt cyto.c1 cells (Supplementary information, Video S2A). However, the cyto.c release and mitochondrial fragmentation were largely inhibited in the cells expressing non-cleavable cyto.c1 or by z-VAD-fmk (Figure 3B and Supplementary information, Video S2B and S2C). At the same time, the PARP cleavage was observed in the wt cyto.c1, but not in the non-cleavable cyto.c1 cells by STS (Figure 3C). These data thus identified that the cleavage of cyto.c1 is a critical step for cells to undergo apoptosis. This effect is specific, as mutation of D128 or D157 to alanine does not confer the resistance of cyto.c1 to casp.3 cleavage (Figure 2D) and these cells are still sensitive to STS-induced apoptosis (Figure 3A).

To further ascertain the effect of cyto.c1 cleavage on apoptosis, we used shRNA to specifically knock down the endogenous cyto.c1 and then reintroduced the RNAi-resistant wt or non-cleavable mouse cyto.c1 into the cells. Knockdown of the endogenous cyto.c1 resulted in apoptosis inhibition (Figure 3D). Expression of the mouse wt cyto.c1, but not the non-cleavable cyto.c1, in the shRNA-knocking down HeLa cells restored the cell sensitivity towards apoptosis (Figure 3D). These results strongly support that cyto.c1 is a substrate of casp.3 in vivo and the cleavage of cyto.c1 is critical for the progression of apoptotic phenotypes.

HeLa cells expressing non-cleavable cyto.c1 maintain mitochondrial morphology and functions

Mitochondria maintain their unique morphology for their functions and will undergo extensive morphological changes including mitochondrial swelling, remodeling of inner membrane and fragmentation during apoptosis. A line of evidence has suggested that these changes could be caspase dependent although the underlying mechanism is not clear. We thus examined if the cyto.c1 cleavage is associated with mitochondrial morphology and functions. As shown in Figure 3B (right panel), STS was able to effectively induce the fragmentation of mitochondria in HeLa cells expressing wt, not non-cleavable cyto.c1. In addition, we found that the mitochondrial fragmentation could be inhibited by N-acetyl cysteine (NAC) (Supplementary information, Figure S3) suggesting that ROS, likely to be generated from the impaired mitochondrial respiratory chain, involves mitochondrial fragmentation.

We next examined the effects of the expression of wt and non-cleavable cyto.c1 on mitochondrial respiration during apoptosis. Upon STS treatment, the state IV respiration was maintained while there was significant reduction of state III respiration. The respiratory control ratio (RCR) in the cells expressing wt, but not non-cleavable cyto.c1, was remarkably decreased in the presence of STS. Interestingly, the ATP synthase activity in both cell types was decreased, but the cellular NADH levels in both cells were not affected upon STS treatment. Therefore, it seemed that the coupling of mitochondrial electron transfer and ATP generation was compromised while the cleavage of cyto.c1 was occurring. Accordingly, non-cleavable cyto.c1 prevented the loss of mitochondrial physiology and functions to maintain their viability when treated with STS (Table 1). These results demonstrated that the cleavage of cyto.c1 resulted in the metabolic catastrophe.

Table 1. Effect of the mitochondrial respiratory, cell oxidative phosphorylation and aerobic glycolysis by STS.

  RCR (control) RCR (STS) ATP synthase activity1 (control) ATP synthase activity1 (STS) NADH2 (control) NADH2 (STS)
Mock 2.8 ± 0.3 1.6 ± 0.5 108 ± 8.1 63 ± 6.7 1.2 ± 0.08 1.0 ± 0.20
wt Cyt.C1 2.8 ± 0.5 1.5 ± 0.6 109 ± 5.7 64 ± 3.2 1.2 ± 0.16 1.1 ± 0.15
D106A Cyt.C1 3.5 ± 0.2 3.2 ± 0.3 123 ± 10.1 82 ± 4.9 1.6 ± 0.14 1.6 ± 0.21
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Cells were cultured in the presence or absence of STS (0.1 μM) for 12 h and collected. The cellular NADH level and mitochondrial ATP synthase activity were detected as described in Materials and Methods. Data are expressed as mean ± SEM.

1nmol/min per mg protein

2Fluorescence (arbitory units)/106 cell.

To further elucidate the effect of the interaction between cyto.c1 and cyto.c on the cyto.c release, we used rho zero cells, which are deficient in mtDNA and lack electron transfer and ROS production in mitochondria. Interestingly, we were still able to detect casp.3 activation and its cleavage of cyto.c1 (Supplementary information, Figure S4), suggesting that the cyto.c release could occur in the absence of mitochondrial respiration and ROS. This further supports that the cleavage of cyto.c1 is important for cyto.c release. Collectively, these results demonstrated that the cleavage of cyto.c1 at D106 is critical for cyto.c release, which may represent the critical step for the release of cyto.c positively feedback to attack mitochondria to amplify cyto.c release as we previously proposed.

z-VAD-fmk inhibits cyto.c release and mitochondrial fragmentation even when casp.3 is partially activated

Our data collectively have shown that cyto.c1 cleavage by casp.3 is important for the apoptotic events such as cyto.c release and mitochondrial fragmentation. To test that there is a positive feedback loop for caspase amplification of cyto.c release via attacking mitochondria, we treated the cells with STS for 3 or 6 h, which allows certain levels of activation of caspases and then monitored the cyto.c release in the presence or absence of z-VAD-fmk (Figure 4). Although casp.3 was activated at 3 and 6 h in the cells, z-VAD-fmk can still largely block further cyto.c release (Figure 4 and Supplementary information, Videos S2 and S3). Mitochondrial fragmentation was also inhibited by z-VAD-fmk, even 3 and 6 h after STS treatment (Figure 4 and Supplementary information, Video S3B and S3C). These data strongly suggest that caspase could feedback attack mitochondria for the progression of apoptosis.

Figure 4.

Figure 4

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The z-VAD-fmk prevents cyto.c1 cleavage and inhibits cyto.c release and mitochondrial fragmentation. (A) Representative images from the video recording showing that z-VAD-fmk inhibits cyto.c release when added at 3 or 6 h after STS treatment. The GFP-cyto.c/MitoDsRed cells were treated with STS for 0, 3 and 6 h and z-VAD-fmk (100 μM) was added at the indicated times. Time lapse video of cyto.c levels and mitochondrial morphology were conducted for 12 h. Cells treated with STS alone for 12 h (upper). Cells supplemented with z-VAD-fmk after treated with STS for 3 h (middle). Cells supplemented with z-VAD-fmk after treated with STS for 6 h (lower). (B, C) GFP-cyto.c/MitoDsRed cells were first treated by STS for 0, 3 and 6 h and then supplemented with z-VAD. Cells were fixed and analyzed by confocal microscopy at 12 h to determine cyto.c levels and mitochondrial morphology. (D) The z-VAD-fmk partially inhibits cyto.c1 cleavage and casp.3 activation when added at later time points. HeLa cells were treated with 0.1 μM STS for the indicated times and then supplemented with z-VAD-fmk before harvesting at 12 h. Both cyto.c1 cleavage and casp.3 were detected by western blotting.

Truncated cyto.c1 enhances mitochondrial fragmentation

To address if the truncated product of cyto.c1 affects mitochondrial functions and cyto.c release, we transiently expressed myc-tagged wt cyto.c1, truncated cyto.c11-106 and cyto.c1107-325 in HeLa cells. As expected, wt cyto.c1 does not affect mitochondrial morphology. Strikingly, the truncated cyto.c11-106 alone enhanced mitochondrial fragmentation (Figure 5A and 5B) as shown by significantly less staining of mitotracker, indicative of the loss of mitochondrial membrane potential 31. These cells are also more sensitive to STS-induced mitochondrial fragmentation and membrane potential loss (Figure 5A and 5B). Furthermore, we also found that the truncated cyto.c11-106-induced cells death and cyto.c release in the cyto.c1 knock-down (KD) cells (Figure 5C and 5D). However, the truncated cyto.c1107-325 failed to localize at mitochondria (as it lacks mitochondrial-targeting sequence) and had no effect on mitochondrial morphology (data not shown). Therefore, our data clearly showed that truncation of cyto.c1, which affects the interaction of endogenous cyto.c1 with cyto.c, resulted in the impaired mitochondrial respiration and increased ROS for mitochondrial fragmentation.

Figure 5.

Figure 5

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Truncated cyto.c1 affects the mitochondrial morphology. (A) Cells were transfected with wt and truncated cyto.c1 and then exposed to 0.1 μM STS for 6 h. Cyto.c1 expression was detected using an anti-myc primary antibody and FITC-conjugated secondary antibody. Mitochondria were visualized using mitotracker. Mitochondria in cells expressing truncated cyto.c1 are less stained with mitotracker (indicative for the loss of mitochondrial membrane potential) and become fragmented when exposed to STS for 8 h. (B) Statistical results of membrane potential loss (as indicated by the inability to mitotracker staining) and mitochondrial fragmentation in wt and truncated cyto.c11-106 cells. (C) Cyto.c1 KD Cells were transfected with the mouse wt cyto.c1 or truncated cyto.c11-106 for 24 h and treated with STS for 24 h; cyto.c1 expression and cyto.c release were detected using anti-myc (rabbit) and cyto.c (mouse) antibody, followed by incubating with goat anti-rabbit-FITC and donkey anti-mouse-CY3 secondary antibody, respectively. (D) Flow cytometric analysis of apoptosis (Annexin V/PI positive) in the cyto.c1 KD cells expressing wt and truncated cyto.c11-106 following treatment with STS (0.1 μM) for 24 h.

Targeted expression of casp.3 into mitochondrial intermembrane space resulted in cyto.c1 cleavage and cyto.c release

To demonstrate that activated casp.3 in the mitochondrial intermembrane space mediates the cyto.c1 cleavage and mitochondrial dysfunction, we carried out the targeted expression of wt casp.3 into the intermembrane space of mitochondria with the aid of a signaling peptide from Smac (an intermembrane space protein) 32, 33. Our results showed that targeted expression of the signaling peptide tagged-casp.3 resulted in mitochondrial cyto.c release, leading to mitochondrial fragmentation, while expressing the signaling peptide alone had no effect on the mitochondrial morphology (Figure 6A-6C). Concomitantly, cyto.c1 was cleaved at 12 h after transfection when the activity of casp.3 could be detected (Figure 6D). These events can be blocked by z-VAD-fmk, suggesting that the mitochondrial phenotypes were dependent on the activated casp.3 in the intermembrane space. More importantly, mitochondria and cell death in cells with the non-cleavable cyto.c1 were not affected by the expression of mitochondria-targeted casp.3 (Figure 6B). These data strongly support that activated casp.3 in the intermembrane space of mitochondria is responsible for the cyto.c1 cleavage and subsequent mitochondrial dysfunction and cell death.

Figure 6.

Figure 6

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Targeted expression of casp.3 into mitochondrial intermembrane space resulted in cyto.c1 cleavage and cyto.c release. (A) Cells were transfected with the Smac signaling peptide-tagged casp.3 (Smac-casp.3) in the absence or presence of z-AVD-fmk, fixed and Smac-casp.3 expression was detected by rabbit c-myc and a FITC-conjugated rabbit secondary antibody. (B) The z-VAD-fmk and non-cleavable cyto.c1 inhibited cell death and mitochondrial fragmentation. Statistical analysis showing that Smac-casp.3 induced cell death and mitochondrial fragmentation in the wt, non-cleavable cyto.c1 and HeLa cells pre-treated with z-AVD-fmk. (C) Smac-casp.3 induced cyto.c release from mitochondria. Mitochondria and cytosol were isolated from cells transfected with Smac-casp.3 for 0, 6, 12, 18 and 24 h, and cell lyastes were subjected to immunoblotting analysis. (D) Smac-casp.3 induced cyto.c1 cleavage. Cells were transfected with Smac-casp.3 in the absence or presence of 1 z-AVD-fmk for 12 h, casp.3 activation and cyto.c1 cleavage were detected by anti-casp.3 and anti-cyto.c1 antibody, respectively. (E) Model on how cyto.c1 cleavage by casp.3 affects cyto.c release. The cytochrome bc1 complex is the central component of the oxidative respiratory reaction chain that oxidizes ubiquinol and reduces cyto.c. Casp.3 cleavage of cyto.c1 disrupts electron transport chain leading to the increase of ROS, ample release of cyto.c, the loss of mitochondrial membrane potential and mitochondrial function for ATP generation (lower).

Discussion

Our current study identified cyto.c1 as a novel substrate for casp.3. We demonstrated that the cleavage of cyto.c1 caused mitochondrial catastrophe as manifested by impaired mitochondrial ATP generation, the increase of ROS and profound mitochondrial fragmentation. The cleavage could disrupt the interaction of bc1 complex with cyto.c and the electron transfer between bc1 complex and complex IV, resulting in further amplification of mitochondrial cyto.c release and subsequent metabolic catastrophe (Figure 6E). Our data clearly showed that mitochondrial dysfunction induced by caspase feedback attack is important for the progression of apoptosis.

Our results provide a new mechanism for how caspases feedback to amplify cyto.c release and the progression of apoptosis. Casp.3 was activated and indeed translocated into mitochondria following apoptotic stresses. Intriguingly, targeted expression of casp.3 in the mitochondrial intermembrane space could faithfully reproduce the mitochondrial catastrophic phenotypes and cause cyto.c1 cleavage and cyto.c release from mitochondria. Importantly, caspase inhibitor abrogated cyto.c1 cleavage and cyto.c release even when casp.3 was partially activated. These results highlight the importance for the feedback mechanism for cyto.c release and subsequent mitochondrial dysfunctions. It was reported that cyto.c1 works as a homodimer in the bc1 complex 34. Thus, cleavage of both molecules of cyto.c1 in the same complex would result in the loss of its physical interaction with cyto.c and mitochondrial functions. In addition, the cleavage of cyto.c1 could affect the respiration status, ROS production and redox potential of mitochondria that may also contribute to cyto.c release in normal cells 35, 36. It should be noted that reduced form of cyto.c functions as an electron acceptor and physically interacts with cyto.c1. Thus, redox status of cyto.c is important for the retention of cyto.c in place 37, 38. It is interesting to note that, upon apoptotic stimulation, apoptosis was induced and cyto.c1 was cleaved in rho zero cells, which are deficient in mitochondrial DNA-encoding cytochrome b and other key components of bc1 complex in the respiration chain and do not generate mitochondrial ATP or mitochondrial ROS 39, 40. Thus, the cyto.c1 cleavage is important for cyto.c release and cell death.

Previous reports have shown that caspases are located in the mitochondrial intermembrane space 21, 23, 24, 25 and affect mitochondrial ROS production 41. Our data for the first time suggest that the bc1 complex, the central component of the oxidative respiratory reaction chain and a center for free radical generation, could be targeted by casp.3. Several mitochondrial membrane proteins such as Bcl-2 and Mcl-1 have been identified to be cleaved by caspases, leading to the conversion of anti-apoptosis molecules into a Bax-like death promoter and the permeabilization of outer membrane of mitochondria 42, 43. As a result, activated caspases are able to penetrate into the intermembrane space to cleave cyto.c1 for subsequent mitochondrial catastrophe. Previous study has shown that other proteins in mitochondrial respiration complex are also subject to caspase attack. For example, a mitochondrial inner membrane protein termed as p75, a subunit of complex I, is cleaved by activated caspases when mitochondria become permeabilized 41. The cleavage of p75 leads to increase of ROS and loss of plasma membrane integrity without affecting mitochondrial cyto.c release. These results demonstrate that the mitochondrial respiratory chain is one of the major targets by caspases for promoting apoptosis.

The mitochondrial bc1 complex is the major site for intracellular ROS production 6, 34 and genetic defects leading to mutations in the subunits of the bc1 complex result in mitochondrial myopathies and other diseases 44, 45. Mutation of bc1 could also affect the stability of mitochondrial respiration complex I 46. Our results suggest that cyto.c1 is important for mitochondrial morphology and functions. Expression of truncated cyto.c11-106 could also affect mitochondrial phenotype. Knockdown of cyto.c1 by specific shRNA could reduce cell death in mammalian cells. Disruption of the interaction between cyto.c1 and cyto.c by caspase could impair mitochondrial functions and cause mitochondrial catastrophe. Both mitochondrial metabolic catastrophe and abnormal apoptosis are closely associated with a number of pathophysiological conditions such as diabetes, neurodegenerative diseases and cancers 38, 41. Our results offer a fresh understanding of how metabolic catastrophe is causally linked with apoptosis and better understanding of the interplay of these complex processes will be useful to fight these metabolic and aging-related diseases.

Materials and Methods

Materials

Antibodies: Anti-cyto.c and anti-PARP (BD56433, 56362), anti-cyto.c1 (Protein Tech), anti-β-actin (Sigma, a5441), anti-myc (Santa Cruz, sc-40) and anti-casp.3 (Q Chen Lab).

Reagents: Caspase inhibitor z-VAD-fmk (CalBiochem 627610), CaspACETM FITC-VAD-fmk (Promega G7462), PhiPhiLux-G1D2 (Oncoimmunin A304R1G) and Annexin V-FITC kit (Q Chen Lab). All other chemicals were purchased from Sigma unless otherwise specified.

Cell culture

HeLa cells were maintained in DMEM medium supplemented with 10% FBS (Hyclone) and 1% penicillin-streptomycin at 37 °C and 5% CO2. To establish cell lines stably expressing cyto.c1, HeLa cells were transfected with pCDNA4.0-cyto.c1/myc.his plasmid DNA by phosphate calcium and positive clones overexpressing cyto.c1 were selected with 100 μg/ml Zoecin (Invitrogen R250-01).

Isolation of mitochondria

Mitochondria isolation from HeLa cells Cells (5 × 106) were washed twice with ice-cold PBS and kept on ice for 1 h in hypotonic buffer containing 20 mM HEPES-KOH (pH 7.2), 100 mM KCl, 1.5 mM MgCl2, 1 mM EDTA, 1 mM EGTA, 250 mM sucrose and protease inhibitors (1 mM PMSF and DTT, 10 mg/ml aprotinin, leupeptin and pepstatin). The cell suspension was homogenized with a Dounce homogenizer (KONTES, USA) until more than 50% of the cells were positive for trypan blue uptake, the homogenates were centrifuged at 600× g for 5 min and the supernatants were subjected to further centrifugation at 10 000× g for 10 min. The supernatants were then subjected to further ultracentrifugation at 100 000× g for 45 min. The resulting supernatants represent the cytosolic fractions.

Mouse liver mitochondrial isolation Briefly, mouse liver was suspended in 10 ml of MIB buffer (250 mM sucrose, 2 mM HEPES pH7.4, 0.1 mM EDTA and 0.1% BSA) and dissociated using a 15-ml Dounce homogenizer with a tight-fitting Teflon pestle. Mitochondria were isolated by multiple steps of centrifugation in a Sorvall centrifuge with a swinging bucket rotor. The cellular lysates were centrifuged at 600× g for 10 min and the supernatants were centrifuged at 10 000× g for 15 min. The mitochondrial pellets were resuspended in 15 ml of fresh MIB, centrifuged at 1 500× g for 5 min and the supernatant centrifuged at 10 000× g for 10 min. The last two steps were repeated twice. The final pellets were resuspended in 400 μl of ice-cold MIB.

Diagonal gels

SCR preparation HMP (Keilin-Hartree Heart Muscle Preparation) was prepared according to the published method of Keilin and Hartree 47. SCR was purified from HMP according to the published method 48. Protein concentration was determined by the Bradford method.

Isolation of SCR by SDS-PAGE Diagonal gel was prepared according to the published method 39. A volume of 50 μg of SCR proteins was resolved by 12% SDS-PAGE (first dimension). After migration, the lane containing the protein was excised and soaked in 40% EtOH and 10% acetic acid for 10 min, in 30% EtOH for 10 min and then in ultra pure water for 2× 10 min. The lane was then air dried (15-30 min), soaked in buffer A (50 mM Tris-HCl, 150 mM NaCl, 10 mM DTT) with or without 50 μg of active recombinant casp.3 and incubated overnight at 37 °C. The lane was washed in water to remove the excess protease and then incubated at 95 °C for 10 min in loading buffer (50 mM Tris pH 6.8, 2% SDS, 0.1% bromophenol blue, 10% glycerol, 2.5% β-mercaptoethanol). After cooling, the lane was loaded on a second acrylamide gel (15%) and resolved by SDS-PAGE. After migration, the gel was stained using GelCode Blue Stain Reagent (Pierce). Cleaved proteins, which are located under the diagonal, were excised from the gels and identified by MALDI-TOF-MS (AXIMA-CFR TM plus, Japan).

Assay for ROS generation and electron transport chain (ETC) enzyme activities in isolated mitochondria

ROS generation Mitochondrial ROS generation was detected using luminol plus horseradish peroxidase-derived chemiluminescence with the BPCL Ultra-weak luminescence analyzer at 37 °C. The reaction mixtures contained 500 μM luminol, 2.5 units of horseradish peroxidase, 50 mM Na-phosphate buffer pH 7.4, 4 mg/ml c-dHMP and different concentrations of active recombinant casp.3 in a total volume of 1 ml. The luminol plus horseradish peroxidase-derived chemiluminescence was initiated by adding 300 μM NADH as substrate. The integrity of the signal peak reflects the formation of ROS. The correlation between recombinant casp.3 concentration and ROS formations was plotted.

ETC enzyme activity (complex II-III and IV) All the assays were made at 30 °C in 50 mM phosphate buffer (pH 7.4) using mitochondria purified on sucrose gradients. Complex II-III activity was measured by the rate of cyto.c reduction at 550 nm using succinate (160 μM) as the electron donor. The specificity of the reaction was tested by the antimycin-A (20 μM) sensitivity of the reaction. Complex IV activity was measured by the rate of cyto.c oxidation at 550 nm using 5-15 μg proteins and reduced cyto.c at a final concentration of 30 μM. We used an extinction coefficient of 19 M−1 cm−1. The specificity of the reaction was tested by the KCN (4 mM) sensitivity to the reaction.

Determination of intracellular ROS production

ROS production was detected using CM-H2DCFDA, an uncharged, cell-permeable fluorescent probe. When being incubated with the cells, this dye can readily diffuse into cells and is hydrolyzed by intracellular esterases to yield H2DCF, which is trapped within the cells. Then, it is oxidized from the nonfluorescent form to a highly fluorescent compound by the hydrogen peroxide or other low molecular weight peroxides produced in the cells. Thus, the fluorescence intensity is proportional to the amount of peroxide produced by the cells. Exponentially growing cells (1 × 105 cells/ml) were labeled with CM-H2DCFDA (final concentration 2 μM) for 1 h before treatment and washed with PBS. The green fluorescence intensity in the cells was examined by FACS (Becton Dickinson, USA) with excitation at 488 nm. Propidium iodide (PI; final concentration 10 ng/ml) was added 1 min before flow cytometry. To validate the data, 0.1 mM H2O2 was added 1 h before the staining (not shown). The data were analyzed with the Cell Quest software (BD) for the cell population from which apoptotic cells were gated out against PI positively.

Measurement of mitochondrial membrane potential

This assay was performed as described previously 28. Briefly, cells were collected after treated with STS. DiOC6(3) (final concentration 10 nM) was added to 0.2 ml cell suspension (1 × 105 cells/ml) in PBS (pH 7.2) and incubated at 37 °C for 5 min. PI (5 μl of 500 mg/ml stock) was added 30 s before analysis. The data were validated by addition of 10 μM carbonyl cyanide m-chlorophenylhydrazone (CCCP) after 5 min of DiOC6(3) loading.

Oxidative phosphorylation assay

Polarographic measurement of oxidative phosphorylation was performed as previously described 49. Briefly, mitochondrial oxygen uptake was followed with a Clark type electrode (Yellow Springs Instruments, YSI) connected to a chart recorder via YSI Oxygen monitor. The electrode chamber was loaded with 500 μl incubation medium (100 mM KCl, 50 mM MOPS, 1 mM EGTA, 5 mM potassium phosphate, 1 mg/ml defatted BSA) and equilibrated at 30 °C before the oxygen monitor was set to 100% oxygen saturation. The following components were then added sequentially: mitochondria (maximum 100 μg); 25-50 nM ADP, allowing the mitochondria to consume endogenous substrates; either 10 mM ℒ-malate or 20 mM succinate, providing a defined electron donor specific for complex I or II, respectively; 25-100 nM ADP to determine state 3 and state 4 respiration rates.

Analysis of protein expression

Briefly, cells were washed and lysed in buffer containing 150 M NaCl, 25 mM HEPES pH 7.4, 1% CHAPS, 0.25% sodium deoxycholate, 1 mM EGTA, 1 mM DTT, 50 μg/ml trypsin inhibitor, 1 mM PMSF and 10 μg/ml aprotinin, leupeptin and pepstatin. Proteins from total cell lysates were resolved on 12%-15% SDS-PAGE and transferred to a nitrocellulose membrane. The membranes were blocked with 5% nonfat dry milk and 0.1% Tween 20 for 2 h at room temperature and incubated with the indicated antibodies at 4 °C overnight. Immune complexes were detected with HRP-conjugated secondary antibody and visualized by ECL (Pierce).

Flow cytometric assay for Annexin V positivity

Apoptosis was measured using the Annexin V detection kit according to the manufacturer's instruction. Flow cytometric analysis was performed to monitor the green fluorescence of FITC-conjugated Annexin V and the red fluorescence of DNA-bound PI.

Cleavage of cyto.c1 protein

Caspase in vitro cleavage experiments were performed as described previously with modification 42, 43. In brief, 20-50 μg of cell lysate or isolated mitochondria lysate were incubated with 0-200 ng of recombinant casp.3 at 37 °C for 2 h in 50 μl of reaction buffer (100 mM Hepes pH 7.5, 20% glycerol, 0.5 mM EDTA, 10 mM DTT). The reactions were stopped and resolved by 15% SDS-PAGE and western blotted with cyto.c1 antibody 40, 41.

Cell fractionation and in vitro cell-free assay for caspase-induced cyto.c release

Isolated mitochondria (20-50 μg) were incubated in a total volume of 50 μl buffer (250 mM sucrose, 2 mM HEPES, 0.5 mM KH2PO4 and 4.2 mM potassium succinate, pH 7.4) in the presence or absence of recombinant casp.3 for 2 h at 25 °C, followed by centrifugal separation of mitochondria (12 000× g, 10 min at 4 °C). Aliquots of the supernatant (20 μl) were subjected to western blotting. Cyto.c was detected by anti-cyto.c mAb. Equal protein loading was confirmed by immunodetection of cyto.c oxidase subunit IV (COX-IV) or VADC.

siRNA design and transfection

The pSilencer™ 4.1-CMV neo vector were inserted by a DNA fragment encoding a 19-mer hairpin sequence specific to the cyto.c1 mRNA target, a loop sequence separating the two complementary domains and a dinucleotide overhang that can hybridize with the RNA target.

#1: sense: 5′-gatccgctgttcgactatttcccattcaagaga tgggaaatagtcgaacagctta-3′

Anti-sense: c1-rnai1-r: 5′-agcttaagctgttcgactatttcccatctcttgaa tgggaaatagtcgaacagcg-3′

#2: sense: 5′-gatccgatgttgatgatgatggct ttcaagaga agccatcatcatcaacatctta-3′

Anti-sense: 5′-agcttaagatgttgatgatgatggct tctcttgaa agccatcatcatcaacatcg-3′

#3: sense: 5′-gatcc tgaagatggggagatgttc ttcaagaga gaacatctccccatcttcatta-3′

Anti-sense: 5′-agcttaatgaagatggggagatgttc tctcttgaa gaacatctccccatcttcag-3′

The 5′ ends of the two oligonucleotides form the BamH 1 and Hind III restriction site overhangs that facilitate efficient directional cloning into pSilencer 4.1-CMV neo.

HeLa cells in six-well plates were transfected with phosphate calcium method. Cells were collected and lysed with NP40 buffer for immunoblotting with anti-cyto.c1 antibody. Cells were cultured in the G418-containing medium (200-500 μg/ml) to enrich the cells that were successfully transfected. The population for an expected phenotype and/or the expression of the target gene was analyzed.

Construction of Smac signaling peptide-tagged casp.3

Smac is a protein localized in the intermembrane space of mitochondrial. The N-terminal 55 residues serve as the mitochondria targeting sequence 32, 33. The DNA sequence of Smac signaling peptide targeting mitochondrial intermembrane space were fused to the N-terminal of casp.3 by PCR and cloned into pCDNA4TO/myc.his B vector by Kpn I and Xho I.

Acknowledgments

This work was supported by grants from the National Basic Research Program (973 program project, No 2009CB521800 and 2011CB910900), the National Natural Science Foundation of China (No 30910103910) to Q Chen and 973 program project (2010CB912200) to Y Zhu. We thank Prof Richard Flavell (Yale School of Medicine, USA) for his kind supply of caspase 3-deficient MEF cells; Prof Douglas Green (St. Jude Children's Research Hospital, USA) for providing the cyto.c-GFP constructs; Prof Xiaodong Wang (University of Texas Southwestern Medical center, USA), Dr Aimin Zhou (Cleveland State University, USA), Dr Wei-Xing Zong (Stony Brook University, USA), Dr Honggang Wang (H. Lee Moffitt Cancer Center, USA) and Prof Jun Zhou (Nankai University, China) for their critical reading of the manuscript and valuable comments.

Glossary

cyto.c

cytochrome c

cyto.c1

cytochrome c1

SCR

succinate-cyto.c reductase

KD

knock-down

wt

wild type

STS

staurosporine

RCR

respiratory control ratio

NAC

N-Acetyl Cysteine

ATP

adenosine-triphosphate

Apaf-1

apoptotic protease-activating factor 1

ROS

reactive oxygen species

casp.3

caspase 3

Footnotes

(Supplementary information is linked to the online version of the paper on the Cell Research website.)

Supplementary Information

Supplementary information, Figure S1

Cyto.c1 was cleaved in MEF cells, but not in caspase 3-knockout cells.

Click here for additional data file. (117.9KB, pdf)
Supplementary information, Figure S2

Confocal microscopic images caspase activation and mitochondrial morphology following staurosporine treatment.

Click here for additional data file. (104.3KB, pdf)
Supplementary information, Figure S3

NAC prevents the production and mitochondrial fragmentation.

Click here for additional data file. (39.2KB, pdf)
Supplementary information, Figure S4

Cyto.c1 cleavage and caspase activation in rho 206 cells.

Click here for additional data file. (100.3KB, pdf)
Supplementary information, Data S1

Materials and Methods

Click here for additional data file. (12.3KB, pdf)
Supplementary information, Video S1A
Click here for additional data file. (9.5MB, tif)
Supplementary information, Video S1B
Click here for additional data file. (6.6MB, tif)
Supplementary information, Video S1C

Video S1 Caspase activation in wild type and D106A cyto.c1 cells. Time lapse imaging of caspase activation and mitochondrial morphology following staurosporine (0.1 μM) treatment. The simultaneous recording of mitochondrial morphology (red) and fluorescent images of activated caspases (green) was carried out by a ZEISS LSM510 laser scanning confocal microscope system as described in Supplementary information, Data S1 and Figure S3. Confocal images were taken every 3 min for 4-12 h. The time was chosen as we previously showed that caspase is activated at this particular time. Video S1A: cells expressing wild type cyto.c1; Video S1B: cells expressing mutant cyto.c1 D106A; Video S1C: mock cells in the presence of z-VAD (100 μM)

Click here for additional data file. (8.3MB, tif)
Supplementary information, Video S2A
Click here for additional data file. (9.5MB, tif)
Supplementary information, Video S2B
Click here for additional data file. (7.5MB, tif)
Supplementary information, Video S2C

Video S2 GFP-cyto.c release in wild type and D106A cyto.c1 cells. Cell suspensions were transferred to a thermostated chamber with a glass cover-slip bottom, allowed adhering for 24 h, then cells were co-transfected with pEGFP-C3-cyto.c and MitoDsRed (DNA, 10:1) for 36 h before treatment with staurosporine. Cells with GFP-labeled cyto.c correctly located at mitochondria were chosen to perform the time lapse imaging. The simultaneous recording of mitochondrial morphology (mitoDsRed) and GFP-cyto.c (green) were carried out by a ZEISS LSM510 laser scanning confocal microscope system as described in Supplementary information, Data S1. Confocal images were taken every 2 min for 1 h after the addition of staurosporine. Video S2A: cells expressing wild type cyto.c1; Video S2B: cells expressing mutant cyto.c1 D106A; Video S2C: mock cells in the presence of z-VAD (100 μM).

Click here for additional data file. (8.4MB, tif)
Supplementary information, Video S3A
Click here for additional data file. (10.9MB, tif)
Supplementary information, Video S3B

Video S3 z-VAD-fmk can inhibit cyto.c release when added 3 or 6 h after staurosporine treatment. Single clonally cell expressing GFP-cyto.c (pEGFP-C3-cyto.c) and MitoDsRed located in mitochondria was acquired for assay. Cells were treated with 0.1 μM staurosporine for 3 h (A) or 6 h (B) before supplemented with z-VAD (100 μM). The simultaneous recording of mitochondrial morphology (mitoDsred) and GFP-cyto.c (green) were carried out by a ZEISS LSM510 laser scanning confocal microscope system as described in Supplementary information, Data S1. Confocal images were taken every 2 min. Video S3A: z-VAD added at 3 h after staurosporine treatment; Video S3B: z-VAD added at 6 h after staurosporine treatment.

Click here for additional data file. (10.1MB, tif)

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Associated Data

This section collects any data citations, data availability statements, or supplementary materials included in this article.

Supplementary Materials

Supplementary information, Figure S1

Cyto.c1 was cleaved in MEF cells, but not in caspase 3-knockout cells.

Click here for additional data file. (117.9KB, pdf)
Supplementary information, Figure S2

Confocal microscopic images caspase activation and mitochondrial morphology following staurosporine treatment.

Click here for additional data file. (104.3KB, pdf)
Supplementary information, Figure S3

NAC prevents the production and mitochondrial fragmentation.

Click here for additional data file. (39.2KB, pdf)
Supplementary information, Figure S4

Cyto.c1 cleavage and caspase activation in rho 206 cells.

Click here for additional data file. (100.3KB, pdf)
Supplementary information, Data S1

Materials and Methods

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Supplementary information, Video S1A
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Supplementary information, Video S1B
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Supplementary information, Video S1C

Video S1 Caspase activation in wild type and D106A cyto.c1 cells. Time lapse imaging of caspase activation and mitochondrial morphology following staurosporine (0.1 μM) treatment. The simultaneous recording of mitochondrial morphology (red) and fluorescent images of activated caspases (green) was carried out by a ZEISS LSM510 laser scanning confocal microscope system as described in Supplementary information, Data S1 and Figure S3. Confocal images were taken every 3 min for 4-12 h. The time was chosen as we previously showed that caspase is activated at this particular time. Video S1A: cells expressing wild type cyto.c1; Video S1B: cells expressing mutant cyto.c1 D106A; Video S1C: mock cells in the presence of z-VAD (100 μM)

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Supplementary information, Video S2A
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Supplementary information, Video S2B
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Supplementary information, Video S2C

Video S2 GFP-cyto.c release in wild type and D106A cyto.c1 cells. Cell suspensions were transferred to a thermostated chamber with a glass cover-slip bottom, allowed adhering for 24 h, then cells were co-transfected with pEGFP-C3-cyto.c and MitoDsRed (DNA, 10:1) for 36 h before treatment with staurosporine. Cells with GFP-labeled cyto.c correctly located at mitochondria were chosen to perform the time lapse imaging. The simultaneous recording of mitochondrial morphology (mitoDsRed) and GFP-cyto.c (green) were carried out by a ZEISS LSM510 laser scanning confocal microscope system as described in Supplementary information, Data S1. Confocal images were taken every 2 min for 1 h after the addition of staurosporine. Video S2A: cells expressing wild type cyto.c1; Video S2B: cells expressing mutant cyto.c1 D106A; Video S2C: mock cells in the presence of z-VAD (100 μM).

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Supplementary information, Video S3A
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Supplementary information, Video S3B

Video S3 z-VAD-fmk can inhibit cyto.c release when added 3 or 6 h after staurosporine treatment. Single clonally cell expressing GFP-cyto.c (pEGFP-C3-cyto.c) and MitoDsRed located in mitochondria was acquired for assay. Cells were treated with 0.1 μM staurosporine for 3 h (A) or 6 h (B) before supplemented with z-VAD (100 μM). The simultaneous recording of mitochondrial morphology (mitoDsred) and GFP-cyto.c (green) were carried out by a ZEISS LSM510 laser scanning confocal microscope system as described in Supplementary information, Data S1. Confocal images were taken every 2 min. Video S3A: z-VAD added at 3 h after staurosporine treatment; Video S3B: z-VAD added at 6 h after staurosporine treatment.

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