A number of diseases are due to lysosomal destabilization, which results in damaging cell loss. To investigate the mechanisms of lysosomal cell death, we characterized the cytotoxic action of two widely used quinolone antibiotics: ciprofloxacin (CPX) or norfloxacin (NFX). CPX or NFX plus UV light (NFX*) induce lysosomal membrane permeabilization (LMP), as detected by the release of cathepsins from lysosomes. Inhibition of the lysosomal accumulation of CPX or NFX suppresses their capacity to induce LMP and to kill cells. CPX- or NFX-triggered LMP results in caspase-independent cell death, with hallmarks of apoptosis such as chromatin condensation and phosphatidylserine exposure on the plasma membrane. LMP triggers mitochondrial membrane permeabilization (MMP), as detected by the release of cytochrome c. Both CPX and NFX* cause Bax and Bak to adopt their apoptotic conformation and to insert into mitochondrial membranes. Bax−/− Bak−/− double knockout cells fail to undergo MMP and cell death in response to CPX- or NFX-induced LMP. The single knockout of Bax or Bak (but not Bid) or the transfection-enforced expression of mitochondrion-targeted (but not endoplasmic reticulum–targeted) Bcl-2 conferred protection against CPX (but not NFX*)-induced MMP and death. Altogether, our data indicate that mitochondria are indispensable for cell death initiated by lysosomal destabilization.
The ultimate morphological and biochemical features of apoptotic cells are largely independent of the death-initiating pathway, a fact that led to the concept of the “central executioner,” a self-amplifying device that involves caspase activation cascades and/or mitochondrial membrane permeabilization (MMP;*
Abbreviations used in this paper: AO, acridine orange; Baf A1, Bafilomycin A1; CPX, ciprofloxacin; ΔΨm, mitochondrial transmembrane potential; DAPI, 4′,6-diamidino-2-phenylindole; DiOC6(3), 3,3′ dihexyloxacarbocyanine iodide; DKO, double knockout; GFP, green fluorescent protein; JC-1, 5,5′,6,6′-tetrachloro-1,1′,3,3′-tetraethylbenzimidazolylcarbocyanine iodide; LMP, lysosomal membrane permeabilization; MEF, mouse embryonic fibroblasts; MMP, mitochondrial membrane permeabilization; NFX, norfloxacin; NFX*, NFX plus UV light; PI, propidium iodide; PS, phosphatidylserine; ROS, reactive oxygen species; z-FA-fmk, N-benzyloxycarbonyl-Phe-Ala-fluoromethylketone; z-VAD-fmk, N-benzyloxycarbonyl-Val-Ala-Asp-fluoromethylketone.
Lysosomes, which have been referred to as “suicide bags,” notoriously contribute to autophagic cell death (also called “type II” cell death; references 7–9). Recent observations suggest that p53 can trigger a primary lysosomal destabilization that contributes to cell death via apoptosis (10). In pro-oxidant–induced apoptosis, the release of cathepsin D from lysosomes reportedly precedes the release of cytochrome c from mitochondria (11). Ceramide generated by the lysosomal sphingomyelinase can trigger the proteolytic autoactivation of cathepsin D (12). Hepatocytes from cathepsin B knockout mice are relatively resistant to TNF-α–induced apoptosis (13), and cathepsin B participates in TNF-α-induced, caspase-independent cell death of WEHI-S cells (14). Enzymatic defects resulting in lysosomal destabilization can cause unwarranted (possibly apoptotic) cell loss, in particular in the central nervous system. This applies to clinically important diseases such as Sandhoff disease, Gaucher disease, Farber's disease, Niemann Picks' disease, and neural ceroid lipofuscinosis (4).
In spite of this wealth of information, it is currently unknown to what extent MMP is required for cell death initiated at the lysosomal level. On theoretical grounds, two possibilities could be envisioned. On the one hand, MMP could be a rate-limiting step of lysosome-initiated death, which would be in line with the idea that MMP would be part of the “central executer” (1) or “gateway to death” (5). On the other hand, some data suggest that lysosomal destabilization and cathepsins might trigger cell death via novel, MMP-independent pathways, e.g., via direct cathepsin effects on the nucleus (9, 15, 16).
Lysosomotropic agents are lipophilic bases that accumulate in the lysosomal lumen and can exert detergent-like or local phototoxic effects on lysosomal membranes. Two quinolone antibiotics, norfloxacin (NFX) and ciprofloxacin (CFX), which are used on millions of patients each year, are lysosomotropic and can induce apoptosis either in the presence (NFX) or absence (CFX) of a low dose of UV light (17–19). This property may explain the unwarranted cytotoxicity of such compounds (and, in particular, the deleterious effect of NFX medication plus sunlight exposure) and lead to the proposal that quinolone antibiotics could be used for cancer therapy (19).
Here, we show that NFX and CFX kill cells through a lysosomal mechanism. Using NFX and CFX as specific tools for the organelle-specific initiation of cell death, we addressed the functional hierarchy between lysosomes, MMP, and caspases. Our results indicate that MMP mediated by Bax and/or Bak is strictly required for the induction of cell death through a caspase-independent pathway initially triggered at the lysosomal level.
Materials And Methods
Cell Lines, Culture Conditions, and Transfection.
HeLa cells were stably transfected with pcDNA3.1 control vector (Neo), with human Bcl-2 (Bcl-2) or the cytomegalovirus UL37 exon 1 gene (vMIA, provided by Dr. V. Goldmacher, ImmunoGen, Cambridge, MA; reference 20), or a histone H2B–green fluorescent protein (GFP) fusion construct (H2B-GFP, a gift from Dr. G.M. Wahl, Salk Institute, La Jolla, CA; reference 21). Rat-1/myc fibroblasts (provided by Dr. D. Andrews, McMaster University, Hamilton, Canada) were stably transfected with pRc/CMV-based plasmids (Neo) and constitutively express human Bcl-2, mitochondrion-targeted Bcl-2 acta, and ER-targeted Bcl2-cb5 (22, 23). Cells were cultured in DMEM supplemented with 10% FCS, 1 mM of pyruvate, 10 mM Hepes, and 100 U/ml penicillin/streptomycin at 37°C under 5% CO2. SV40-transformed MEF, whose genotype was either wild type, Bax−/−, Bak−/−, Bax−/− Bak−/− double knockout (DKO), Bid+/+, or Bid−/− (provided by Dr. S. Korsmeyer, Harvard Medical School, Boston, MA), were cultivated in IMDM (Life Technologies) supplemented with 20% FCS, 1× NEAA (Sigma-Aldrich), and 100 U/ml penicillin/streptomycin at 37°C under 5% CO2 (5). MEF from wild-type (WT), cathepsin B–deficient (24), cathepsin L–deficient (25), cathepsin S–deficient (26), and cathepsin D–deficient mice (provided by Dr. M. Boes, Harvard Medical School, Boston, MA; reference 24) were immortalized with SV40 (27). Transfection with pcDNA3.1 vector only or p53-responsive enhanced GFP plasmid (a gift from K. Wiman, Karolinska Cancer Center, Stockholm, Sweden) was performed by electroporation 24 h before induction of cell death. The p53-responsive GFP plasmid was generated by replacing the luciferase gene in PG13PY Luc (a luciferase construct containing 13 repeats of the p53-binding oligonucleotide 5′-CCTGCCCTGGGACTTGCCTGG-3′, a gift from Dr. B. Vogelstein, Johns Hopkins University, Baltimore, MD) with an EcoA7III–MluI fragment from pEGFP-C1. DAP kinase cDNA and its mutants were a gift from A. Kimchi (Weizmann Institute, Rehovot, Israel).
Cell Death Induction and Inhibition.
Cells were cultured with CPX (standard dose 350 μg/ml, Bayer), chloroquine (Sigma-Aldrich), 1 μM staurosporine, 100 μM etoposide, 200 μM cisplatin (Sigma-Aldrich), or a combination of anti-CD95 (clone 7C11, 100 ng/ml for 15 h; Immunotech) and 35 μM cycloheximide. Serum withdrawal was performed for 24 h. Alternatively, cells were incubated with NFX (standard dose 10 μg/ml; Sigma-Aldrich) for 1 h and irradiated with a UV lamp (365 ± 5 nm) at 12 J/cm2. 0.1 μM Bafilomycin A1 (Baf A1, Sigma-Aldrich), 100 μM z-FA-fmk, N-benzyloxycarbonyl-Phe-Ala-fluoromethylketone; 100 μM z-VAD-fmk, N-benzyloxycarbonyl-Val-Ala-Asp-fluoromethylketone (Bachem), 10 μM CA-074-Me (Peptides International), 100 μM of pepstatin A (Sigma-Aldrich), 10 μM of cyclic pifthrin-α (Calbiochem), 10 mM GSH ethyl ester (Sigma-Aldrich), or 100 μM MnTBAP (Calbiochem) were added 1 h before induction of cell death. MEF (107 in 150 μl RPMI 1640) were electroporated (with a Bio-Rad gene pulser set at 250 V and 960 μF) with 10 μg vector only (pcDNA3.1), WT DAP kinase or its constitutively active or inactive mutants (DAP kinase ΔCaM or DAP kinase ΔDD, respectively; reference 28), together with 10 μg pDS-Red1-mito vector (CLONTECH Laboratories, Inc.), for the identification of transfected (∼50%) cells.
Lysosomal Stability Assessment.
To determine the intracellular localization of NFX and CPX, cells cultured on coverslips were loaded with 10 μg/ml of the antibiotics and visualized under fluorescence microscopy. To label lysosomes, cells were incubated with 0.5 μM of LysoTracker red (Molecular Probes) for 15 min at 37°C and visualized by fluorescence microscopy (10, 29) or with acridine orange (AO, 5 μM, 30 min, 37°C), followed by determination of the red AO fluorescence by flow cytometry (30).
We used 40 nM 3, 3′ dihexyloxacarbocyanine iodide (DiOC6(3)) for ΔΨm quantification, 1 μg/ml propidium iodide (PI) for determination of cell viability, 10 μM hydroethidine ( Molecular Probes) for the determination of superoxide anion generation, and Annexin V conjugated with fluorescein isothiocyanate kit (Bender Medsystems) for the assessment of phosphatidylserine (PS) exposure (31). Quantification of DNA content was performed on ethanol-fixed cells which were stained with 4′,6-diamidino-2-phenylindole (DAPI; 2.5 μg/ml; Molecular Probes) for 30 min at 37°C.
Light Microscopy and Immunofluorescence.
Cells cultured on coverslips were stained with 3 μM 5,5′,6,6′-tetrachloro-1,1′,3,3′-tetraethylbenzimidazolylcarbocyanine iodide (JC-1; Molecular Probes) and 2 μM Hoechst 33342 (Sigma-Aldrich), followed by fluorescence microscopic assessment. Alternatively, cells were fixed with paraformaldehyde (4% wt/vol) and picric acid (0.19% vol/vol) for immunofluorescence assays (32). Cells were stained for the detection of cytochrome c (mAb 6H2.B4; BD Biosciences), activated Bax (mAb 6A7; BD Biosciences), activated Bak (mAb Ab-1 specific for the NH2 terminus, Oncogene Research Products), cathepsin B (Calbiochem), and monoclonal anti–cathepsin D (clone CTD-19; Sigma-Aldrich); all were detected by a goat anti–mouse or goat anti–rabbit IgG conjugated with Alexa® Fluor (Molecular Probes; reference 33). Giemsa stainings were performed with a kit from Sigma-Aldrich.
Cells were fixed for 1 h at 4°C in 2.5% glutaraldehyde in phosphate buffer (pH 7.4), washed, and fixed again in 2% osmium tetroxide before embedding in Epon. Electron microscopy was performed with an transmission electron microscope (model EM902; Carl Zeiss MicroImaging, Inc.), at 80 kV, on ultrathin sections (80 nm) stained with uranyl acetate and lead citrate.
After the different treatments, cells were lysed for 15 min in 50 mM Hepes, 150 mM NaCl, 5 mM EDTA, and 0.1% NP-40, supplemented with protease inhibitor cocktail (1 mM DTT and 1 mM PMSF; Roche), and centrifuged at 13,000 g for 10 min to remove cell debris. Total protein content was determined with the Bio-Rad DC kit. 40 μg of protein were loaded on a 15% SDS-PAGE. Anti-cleaved caspase-3 antibody (Cell Signaling Technology) was used to determine caspase-3 activation and anti–glyceraldehyde-3-phosphate dehydrogenase (Chemicon) was used as a loading control.
Results And Discussion
NFX and CPX Induce Permeabilization of Lysosomal Membranes.
Based on the intrinsic low-level fluorescence of NFX and CPX (34), we determined their subcellular localization. Both agents were found enriched in the nucleolus as well as in cytoplasmic vesicles (Fig. 1
A). Inhibition of the lysosomal vacuolar H+ ATPase with Baf A1 abolished the cytoplasmic (but not the nucleolar) accumulation of NFX and CPX, indicating that the NFX/CPX-containing vesicles are lysosomes (Fig. 1 A). Cells exposed to NFX or to a low dose of UV light alone exhibited normal staining, with two acidophilic dyes specifically labeling lysosomes: namely a punctate lysosomal staining with LysoTracker red (Fig. 1 B) and a marked red fluorescence with AO (Fig. 1 C). When NFX was combined with UV light (NFX*), an immediate phototoxic effect was noted at the level of lysosomes, leading to the loss of the punctate LysoTracker red staining pattern (Fig. 1 B) and a diminution of the red AO fluorescence (Fig. 1 C). NFX*, but not NFX or UV light alone, caused lysosomes to release cathepsins B and D into the cytosol (Fig. 1, D and E). Similarly, CPX reduced LysoTracker incorporation (Fig. 1 B), attenuated AO staining (Fig. 1 C), and led to the translocation of cathepsins B and D (Fig. 1, D and E). In conclusion, NFX mediates the UV-elicited (photodynamic) permeabilization of lysosomal membranes, and CPX alone exerts similar effects.
* and CPX Induce Caspase-independent Cell Death with MMP.
The combination of NFX and UV light (NFX*), as well as CPX alone, induced several hallmarks of apoptosis, in particular the exposure of residues on the plasma membrane surface (Fig. 2, A and B)
and the loss of nuclear DNA (Fig. 2 C). Although CPX caused proteolytic maturation of caspase-3, NFX* failed to induce caspase activation, as determined by immunoblots (Fig. 2 D). Importantly, treatment with the pan-caspase inhibitor z-VAD-fmk failed to prevent the induction of chromatin condensation by NFX* or CPX, as determined by Giemsa staining (Fig. 2 E) as well as in unfixed cells engineered to stably express a histone H2B-GFP chimera, allowing for the constant monitoring of chromatin structure (Fig. 2, F and H). This chromatin condensation was less pronounced as that induced by CD95 cross-linking (which, however, was fully inhibited by z-VAD-fmk) (Fig. 2, E, F, and H), and was of a more peripheral type, as determined by electron microscopy (Fig. 2 G). z-VAD-fmk failed to prevent PS exposure induced by NFX* or CPX (Fig. 2 I). NFX* and CPX induced signs of MMP such as the dissipation of ΔΨm, measured as a reduction of the DiOC6(3) incorporation (Fig. 3, A and B)
or a spectral red–green shift in the fluorescence of JC-1 (Fig. 3 C), and the mitochondrial release of cytochrome c (Fig. 3 D). Again, z-VAD-fmk failed to affect the signs of MMP induced by NFX* or CPX (Fig. 3 E). The population of cells having released cytochrome c from mitochondria constituted a subensemble of NFX*- or CPX-treated cells with diffuse cathepsin B staining (Fig. 3 F), indicating that MMP occurs after lysosomal membrane permeabilization (LMP). Baf A1 inhibited all hallmarks of cell death induced by NFX* or CPX: loss of the ΔΨm (Fig. 4
Lysosomal Damage Triggers MMP and Cell Death via Bax and Bak.
Both NFX* and CPX induced a conformational change of Bax and Bak (detectable with monoclonal antibodies specific for the NH2 terminus of these molecules), which are exposed only in the “apoptotic conformation” (35, 36). Both NFX* and CPX treatment resulted in a punctate cytoplasmic staining of apoptotic Bax and Bak (Fig. 5
A), which were found to colocalize with the mitochondrial marker Hsp60 (not depicted). The activation of Bax and Bak occurs after LMP (as assessed by measuring the LysoTracker red incorporation and cathepsin B release), but before the mitochondrial release of cytochrome c and before caspase-3–activation (Fig. 5, B and C). These alterations were not due to transcriptional activation of p53 because NFX* and CPX (in contrast to the positive control etoposide) failed to induce a p53-inducible GFP reporter gene (Fig. 5 D). Moreover, NFX*- and CPX-induced MMP and cell death were not inhibited by pifithrin-α, a chemical inhibitor of p53-mediated transactivation (Fig. 5 E) or cycloheximide, a general inhibitor of protein synthesis (not depicted). To directly address the contribution of Bax and Bak to cell death induced by lysomotropic agents, we took advantage of SV40–immortalized MEF lacking Bax, Bak, Bid, or both Bax and Bak. Bax−/−Bak−/− DKO were found to be profoundly resistant to the induction of MMP and PS exposure by NFX* or CPX (Fig. 6
A). Only the DKO of Bax and Bak led to cytoprotection against NFX* (Fig. 6 B). In contrast, the absence of either Bax or Bak (but not Bid) was sufficient to prevent cell death induction by CPX (Fig. 6 B). WT and Bax−/−Bak−/− cells exposed to CPX or NFX* underwent a similar degree of lysosomal disruption, as measured with cathepsin B immunostaining (Fig. 6 C). However, Bax−/− Bak−/− cells manifested much less diffuse cytochrome c staining induced by CPX or NFX*, as compared with controls (Fig. 6 C). The knockout of the genes coding for cathepsin B, D, L, or S and several cathepsin inhibitors failed to prevent CPX- or NFX-induced MMP and cell death (Fig. 6, D and E). Altogether, these data demonstrate that Bax and/or Bak, but not cathepsins, control cell death induced by lysosomotropic agents.
Mitochondrial Bcl-2 and vMIA Selectively Inhibit CPX-mediated MMP and Cell Death.
HeLa cells stably transfected with Bcl-2 or vMIA, a cytomegalovirus-encoded protein that interacts with the mitochondrial adenine nucleotide translocase (20), exhibited a relative resistance to the induction of ΔΨm loss and cell death by CPX but not by NFX* (Fig. 7
A). Bcl-2 specifically targeted to the mitochondrial outer membrane (Bcl-2 acta) was as efficient as WT Bcl-2 in inhibiting CPX-induced MMP and cell killing (Fig. 7 B). In contrast, ER-targeted Bcl-2 (Bcl-2 cathepsin B5; references 22, 23) failed to antagonize CPX (Fig. 7 B). Bcl-2 and vMIA failed to antagonize the dissipation of LysoTracker red staining by CPX (Fig. 7 C). Thus, Bcl-2 and vMIA inhibit CPX but not NFX*-induced cell death at the mitochondrial level.
Involvement of Reactive Oxygen Species (ROS) as Mediators of MMP in NFX
*-induced Cell Death.
The NFX*-induced ΔΨm loss was preceded by an increase in ROS production (as quantified by the ROS-mediated conversion of hydroethidine into the fluorescent product ethidium), whereas CPX-induced ΔΨm loss occurred before ROS production increased (Fig. 8
A). Furthermore, the antioxidants glutathione ethyl ester and MnTBAP prevented NFX*-induced MMP, ROS generation, PS exposure, and cell death, yet had no effect on CPX-induced cell death (Fig. 8, B and C). MnTBAP also inhibited the NFX-induced apoptotic conformation of Bax, yet had no significant effect on CPX-induced Bax activation (Fig. 8 D). The antioxidant partially (∼60%) inhibited the NFX* (but not the CPX)-induced cathepsin B relocalization (Fig. 8 E). Thus, NFX* induces cell death through a photodynamic effect involving ROS upstream of MMP, whereas ROS are not involved in CPX-induced MMP.
MMP Is a General Requirement for Lysosome-initiated Cell Death.
As shown in Fig. 9
A, the cytotoxic effect of chloroquine, yet another lysosomotropic drug, is abolished by either Baf A1 or by the DKO of Bax and Bak. The absence of Bax and Bak also inhibited the ΔΨm loss (Fig. 9 A), the release of cytochrome c, and chromatin condensation induced by chloroquine, yet had no effect on the translocation of cathepsin B (Fig. 9 B). The constitutively active DAP kinase (DAP kinase ΔCaM) has been shown to stimulate a lysosomal/autophagic cell death pathway, when overexpressed in HeLa cells (28). DAP kinase ΔCaM (but not WT DAP kinase or the inactive DAP kinase ΔDD mutant) induces a ΔΨm loss and kills WT MEF, yet has no major effect on Bax−/− Bak−/− MEF. These findings confirm that Bax/Bak-dependent MMP is involved in lysosome-triggered cell death.
We report here the unexpected finding that MMP occurs downstream of LMP, as a down-stream rate-limiting step of cellular demise, based on several signs of evidence. First, LMP is detectable within a few hours after NFX* or CPX treatment, whereas MMP appears later (Figs. 1 and 3 and Fig. 5, B and C). Second, cells with signs of MMP (e.g., cytochrome c release) are a sub-ensemble of cells with signs of LMP (e.g., cathepsin B release), not vice versa (Fig. 3). Third, inhibition of LMP with Baf A1 suppresses MMP (Fig. 4), whereas prevention of MMP by the Bax/Bak DKO, Bcl-2, or vMIA does not block LMP (Figs. 6 C, 7 C, and 9 B). Fourth, when MMP is prevented (by deletion of Bax and/or Bak or overexpression of Bcl-2 or vMIA), LMP fails to cause late manifestations of cell death such as PS exposure, (partial) chromatin condensation, and loss of viability (Figs. 6 and 7). Importantly, the evidence placing LMP upstream of MMP has been obtained with three different clinically relevant drugs (NFX*, CPX, and chloroquine), as well as with DAP-kinase, a signal-transducing molecule known to be involved in physiological cell death induction by γ-interferon and TNF-α (Fig. 9; reference 28). Thus, the importance of MMP for LMP-induced cell death appears to be a general phenomenon.
Although these data imply a clear hierarchical relationship between LMP and MMP with regards to cell death induction (Fig. 10)
, the molecular link between LMP and MMP remains elusive. The lysosomal cathepsins B, D, L, and S do not constitute such a link, as shown by the knockout of each of these cathepsins (Fig. 6 E), as well as by pharmacological studies involving cathepsin inhibitors (Fig. 6 D). Moreover, although the proapoptotic Bcl-2–like protein Bid could constitute a link between LMP and MMP (37, 38), Bid clearly does not contribute to MMP induced by CPX or NFX*, as demonstrated by experiments involving Bid−/− cells (Fig. 6 B). p53-mediated effects, which also have been postulated to participate in LMP-induced apoptosis (39, 40), clearly do not participate in CPX- or NFX-induced MMP, which is independent of the transcription of p53 target genes (Fig. 5, D and E). It has been suggested that cathepsin B would directly activate caspase-3 (41) and/or trigger apoptotic chromatin condensation and nuclear DNA loss (15). However, the presence of cathepsin B in the cytosol and in the nucleus clearly is not sufficient to induce cell death, as shown by the fact that Bax−/−Bak−/− cells can release cathepsin from lysosomes, yet fail to translocate cytochrome c and continue to manifest a normal chromatin structure (Figs. 6 C and 9 B).
Clear differences appear in the mechanisms through which NFX* and CPX induce MMP and cell death, the first one involving ROS (as to be expected for a photosensitizer) and the second acting independently from ROS (Fig. 8). Moreover, the NFX-induced MMP was more difficult to be inhibited than CPX-induced MMP. Only the knockout of both Bax and Bak conferred resistance to NFX* (Fig. 6, A and B). The knockout of either Bax or Bak alone, or the overexpression of vMIA, natural Bcl-2, or mitochondrion-targeted Bcl-2 did not attenuate the NFX-triggered MMP and death, whereas all these manipulations did prevent CPX-mediated MMP (Figs. 6 and 7). Although NFX failed to cause the activation of caspase-3, CPX triggered the proteolytic maturation of caspase-3 (Fig. 2 D). However, caspase inhibition did not block cell death in CPX- or NFX-treated cells (Fig. 2, F and G), which is as in line with the notion that caspase-independent death effectors seal the cell's fate in response to lysosomotropic agents. The ROS-inducing property of NFX* may explain why it acts as a stronger MMP inducer, yet as a weaker caspase elicitor than CPX. Indeed, it is known that primary thiol oxidation of mitochondrial proteins (which may result from an oxidative shift in the cellular redox potential) can induce a Bcl-2–refractory MMP (42–44) and that Bcl-2 can even sensitize to (ROS-mediated) photodynamic therapy (45). Moreover, oxidation of critical thiols within the catalytic center of caspases annihilates their latent proteolytic potential and, thus, precludes their (auto)activation (46).
In conclusion, the data reported herein reveal that MMP may be indispensable for cell death initiated at the lysosomal level, thus reenforcing the concept that MMP constitutes a central event in the death-inducing signaling cascade. Based on these results, studies are underway to explore the possibility that prevention of MMP might diminish pathogenic cell loss triggered by primary lysosomal lesions in pathologies as diverse as Gaucher disease, Sandhoff disease, Farber disease, Niemann Pick disease, neuronal ceroid lipofuscinosis, and age-related macular degeneration.
We thank Drs. D. Andrews, M. Boes, S. Korsmeyer, A. Kimchi, V. Goldmacher, K. Wiman, and G.M. Wahl for reagents, and G. Pierron (UMR 1983, Villejuif, France) for electron microscopy.
This work has been supported by a special grant from Ligue Nationale contre le Cancer, as well as grants from the Agence National pour la Recherche sur le SIDA, Fondation pour la Recherche Médicale, and European Commission (QLG1-CT-1999-00739 and QLK3-CT-2002-01956 to G. Kroemer). P. Boya received a fellowship from the European Commission (MCFI-2000-00943). K. Andreau received a Sidaction fellowship.
P. Boya and K. Andreau contributed equally to this work.