Abstract
The apoptotic program incorporates a paracrine component of importance in fostering tissue repair at sites of apoptotic cell deletion. As this paracrine pathway likely bears special importance in maladaptive intercellular communication leading to vascular remodeling, we aimed at further defining the mediators produced by apoptotic endothelial cells (EC), using comparative and functional proteomics. Apoptotic EC were found to release nanovesicles displaying ultrastructural characteristics, protein markers and functional activity that differed from apoptotic blebs. Tumor susceptibility gene 101 and translationally controlled tumor protein (TCTP) were identified in nanovesicle fractions purified from medium conditioned by apoptotic EC and absent from purified apoptotic blebs. Immunogold labeling identified TCTP on the surface of nanovesicles purified from medium conditioned by apoptotic EC and within multivesicular blebs in apoptotic EC. These nanovesicles induced an extracellular signal-regulated kinases 1/2 (ERK 1/2)-dependent antiapoptotic phenotype in vascular smooth muscle cells (VSMC), whereas apoptotic blebs did not display antiapoptotic activity on VSMC. Caspase-3 biochemical inhibition and caspase-3 RNA interference in EC submitted to a proapoptotic stimulus inhibited the release of nanovesicles. Also, TCTP siRNAs in EC attenuated the antiapoptotic activity of purified nanovesicles on VSMC. Collectively, these results identify TCTP-bearing nanovesicles as a novel component of the paracrine apoptotic program of potential importance in vascular repair.
Similar content being viewed by others
Main
Although classically considered a ‘silent’ process, apoptotic cells are known to actively release paracrine mediators that, in turn, control the phagocytosis of apoptotic cells. For example, apoptotic cells release lysophosphatidylcholine, which favors the recruitment of professional phagocytes and the clearance of apoptotic cells.1 They also secrete lactoferrin as a means of promoting the migration of mononuclear leukocytes, while inhibiting the migration of polymorphonuclear leukocytes.2 Recent results suggest that this paracrine response also aims at fostering tissue remodeling and repair. A C-terminal fragment of perlecan (LG3), released as a consequence of cathepsin L translocation from apoptotic endothelial cells (EC), induces Bcl-xl upregulation and resistance to apoptosis in fibroblasts, mesenchymal stem cells and smooth muscle cells, all of which are pivotal to tissue or vascular remodeling and repair.3, 4, 5, 6, 7 Recently, we showed that caspase-3 activation in EC favors the release of connective tissue growth factor (CTGF),8 which induces the differentiation of fibroblasts into myofibroblasts, a mandatory process in all forms of repair. To date, caspase-3 activation has been implicated in the release of most, if not all, mediators secreted by apoptotic cells,1, 2, 6, 8 suggesting that the paracrine response is embedded within the effector phase of apoptosis.
Dysregulation of apoptosis within cellular constituents of the vessel wall is pivotal to most forms of pathological vascular remodeling. Chronic transplant vasculopathy, systemic sclerosis and classical atherosclerosis are all characterized by the enhanced apoptosis of EC and decreased apoptosis of neointimal cells.9, 10 Neointima formation develops initially through the acquisition of a synthetic and antiapoptotic phenotype in neointimal cells associated with extracellular signal-regulated kinases 1/2 (ERK 1/2) activation and Bcl-xl overexpression.11, 12, 13 Mediators produced by apoptotic EC, such as LG3 and CTGF, actively induce ERK 1/2- and/or Bcl-xl-dependent antiapoptotic phenotypes in vascular smooth muscle cells (VSMC), mesenchymal stem cells and myofibroblasts.3, 4, 5, 6, 7, 8 This raises the possibility that a chronic increase in EC apoptosis, resulting in a sustained paracrine response, could contribute to maladaptive vascular repair.
Here, we aim at further characterizing the molecular paracrine signals released by apoptotic EC, with a specific focus on proteins of importance in fostering a neointimal phenotype in VSMC. We used comparative and functional proteomics to identify novel antiapoptotic mediators released by apoptotic EC through caspase-dependent pathways.
Results
Serum starvation induces a pure apoptotic response in EC
To study the secretome of apoptotic EC, human umbilical vein endothelial cells (HUVEC) were rendered apoptotic in vitro by serum starvation (SS) for 4 h, as reported previously.3, 4, 5, 6, 7, 8 In serum-starved EC, the percentage of cells with chromatin condensation in absence of cell membrane permeabilization increased over time, suggesting increased apoptosis (Figure 1a). The absence of lactate dehydrogenase (LDH) release in serum-starved EC was also consistent with absence of cell membrane permeabilization (Figure 1b). Loss of mitochondrial integrity was evident after 2 h of SS (Figure 1c), with concomitant activation of caspase-9 and caspase-3 and poly(ADP-ribose) polymerase (PARP) cleavage (Figure 1d and e). Preincubating EC with the pan-caspase inhibitor (ZVAD-FMK) or with inhibitors of caspase-3 and caspase-9 (DEVD-FMK and LEHD-FMK, respectively) before SS effectively blocked caspase(s) activation, PARP cleavage and chromatin condensation (Figure 1d–g and Supplementary Figure S2a). Cell membrane permeabilization, suggestive of necrosis, was not significantly modulated by ZVAD-FMK, DEVD-FMK or LEHD-FMK compared with the vehicle (dimethylsulfoxide, DMSO) (Figure 1g). Finally, as expected, pan-caspase inhibition in serum-starved EC did not prevent mitochondrial permeabilization (Figure 1c) and did not modulate p53 protein levels (Figure 1h). Collectively, these results demonstrate a pure intrinsic apoptotic response in serum-starved EC.
Characterization of the secretome of apoptotic EC
Serum-free media conditioned by apoptotic and non-apoptotic EC (SSC-Apo and SSC-No-Apo, respectively) were generated by exposing equal EC numbers to either vehicle (DMSO) or ZVAD-FMK for 2 h, followed by medium change and SS for 4 h, as described above and in Figure 2a. Proteins secreted by apoptotic EC downstream of caspase(s) activation were studied through comparison of equal amounts of proteins precipitated from equal volumes of conditioned media cleared of apoptotic blebs and confirmed by flow cytometric analysis (Figure 2b). Proteins from SSC-Apo and SSC-No-Apo were analyzed comparatively, by either two-dimensional-liquid chromatography tandem mass spectrometry (2D-LC-MS/MS) (Figure 2c) or SDS-PAGE LC-MS/MS14 (Figure 2d). The latter revealed a distinct pattern of Coomassie blue protein staining in SSC-Apo compared with SSC-No-Apo. These results are in keeping with our previous work, describing increased protein secretion downstream of caspase(s) activation by apoptotic EC.6 Concomitantly, SSC-Apo was fractionated by fast protein liquid chromatography (FPLC), and the antiapoptotic activity of each fraction was evaluated on VSMC.3 The protein mediators present in fractions with significant antiapoptotic activity were further characterized by SDS-PAGE LC-MS/MS.
To be considered a specific component of the apoptotic secretome, a protein identified by multifaceted screening had to meet the following criteria: (1) it had to be identified by at least two out of the three different MS/MS approaches, (2) it had to be found exclusively in SSC-Apo and (3) it had to be of human origin. Among the 27 proteins meeting the screening criteria (Table 1), only 11 had known secretion signals and 10 had been previously reported as components of exosomal nanovesicles (Table 1). To evaluate whether proteins known to be secreted through nanovesicles were overrepresented in SSC-Apo compared with SSC-No-Apo, the proteomics data were reanalyzed in search of classical nanovesicle (exosome and exosome-like) markers identified at least once by any proteomics strategies in either SSC-Apo or SSC-No-Apo. In addition to the proteins listed in Table 1, twelve exosomal proteins were identified solely in SSC-Apo, including the two highly characteristic exosomal markers (Alix and CD63),15 whereas only two exosomal proteins were found exclusively in SSC-No-Apo (Table 2). These results suggested increased release of nanovesicles by apoptotic EC downstream of caspase(s) activation.
Caspase(s) activation in apoptotic EC fosters the release of antiapoptotic exosome-like nanovesicles
To determine whether apoptosis specifically increases the release of nanovesicle biomarkers over other proteins, levels of Grp96, an endoplasmic reticulum resident protein, and tubulin, a microtubule-associated protein, were evaluated in intracellular protein extracts and corresponding supernatants of serum-starved EC. Grp96 and tubulin intracellular protein levels were stable throughout SS (Figure 3a). Grp96 and tubulin were not recovered in medium conditioned by serum-starved apoptotic EC (Figure 3a), ruling out the possibility of unspecific protein leakage. These results are in keeping with the absence of cell membrane permeabilization in serum-starved EC (Figure 1a and b). However, protein levels of tumor susceptibility gene 101 (TSG 101) and translationally controlled tumor protein (TCTP), two classical markers of exosomal nanovesicles,15, 16, 17, 18 increased over time in media conditioned by serum-starved EC (Figure 3a).
To specifically address the importance of caspase(s) activation in the production of exosomes or exosome-like nanovesicles by apoptotic EC, protein levels of the exosomal marker TCTP were compared in equal volumes of SSC-Apo and SSC-No-Apo conditioned by equal EC numbers (Figure 3b and Supplementary Figure S2b and S3). Elevated TCTP levels were evident in total unfractionated conditioned medium (Total) and in nanovesicle extracts (Exo) of SSC-Apo compared with SSC-No-Apo. Ponceau red staining confirmed augmented protein content in the nanovesicle fraction of SSC-Apo compared with SSC-No-Apo (Figure 3b). In nanovesicle-free supernatant (SN), the TCTP signal was recovered at similar levels in SSC-Apo and SSC-No-Apo (Figure 3b). In SSC-Apo, TCTP was detectable at different molecular weights (∼23, 50 and 75 kDa) in media conditioned by serum-starved EC (Figure 3a–c), in agreement with the SDS-PAGE LC-MS/MS results where TCTP sequences were identified from two bands (Figure 2d*). High-molecular-weight bands likely represent oligomeric forms of TCTP, as reported previously,19, 20 as the addition of a strong reducing agent (TCEP) to SSC-Apo before protein separation decreased the intensity of high-molecular-weight forms and increased the intensity of the 23-kDa band (Figure 3c, middle and left panels). Also, electrophoresis of recombinant TCTP demonstrated the presence of high-molecular-weight bands (Figure 3c, right panel), indicating dimerization. Of note, recombinant TCTP contains a GST tag, therefore, explaining the higher molecular weights of monomeric and oligomeric forms. Known sequences of importance in TCTP oligomerization19 were present within recombinant TCTP. Collectively, these results confirmed that caspase(s) activation in EC enhances the secretion of the nanovesicle marker TCTP.
To confirm the increased release of nanovesicles by apoptotic EC, ultrastructural studies were performed on nanovesicle fractions isolated from SSC-Apo (Figure 3d). Immunogold labeling revealed the presence of TCTP on nanovesicles of 30–100 nm released by apoptotic EC (Figure 3d) and within multivesicular bodies (MVB) in apoptotic EC (Supplementary Figure S1a). Morphometric quantification of MVB-like structures in apoptotic and non-apoptotic EC demonstrated a 7-fold increase in the volume density of MVB-like structures within apoptotic EC (Supplementary Figure S1b). These data suggested that TCTP-bearing nanovesicles produced by apoptotic EC originated, at least in part, from MVB, consistent with the classical pathways of exosomal nanovesicle formation.
Exosome-like nanovesicles released by apoptotic EC have an antiapoptotic function
We then evaluated whether exosome-like nanovesicles participate in the antiapoptotic activity of the endothelial apoptotic secretome. Equal volumes of SSC-Apo and SSC-No-Apo were ultracentrifuged, supernatants were collected and exosomal pellets were resuspended in the initial volume of serum-free medium. Total unfractionated SSC-Apo and the corresponding supernatant and exosomal fraction significantly inhibited VSMC apoptosis compared with an equal volume of SSC-No-Apo (Figure 3e and Supplementary Figure S1c).
We also considered the possibility that exosome-like nanovesicles produced by apoptotic EC represent unusually small apoptotic blebs. In that event, the functional activity of apoptotic blebs and exosome-like nanovesicles should be similar. Apoptotic blebs were purified by centrifugation from SSC-Apo, and depletion was confirmed by flow cytometry (Figure 2b). VSMC exposed to unfractionated SSC-Apo (Total) or to nanovesicle fractions resuspended in the initial volume of serum-free medium mounted a significant antiapoptotic response as compared with SSC-No-Apo (Figure 3e). However, VSMC exposed to apoptotic blebs resuspended in the initial volume of serum-free medium failed to develop an antiapoptotic response, whereas VSMC exposed to SSC-Apo depleted of apoptotic blebs did so (Figure 3f). Also, TCTP and TSG 101 levels were undetectable in apoptotic blebs isolated from SSC-Apo, whereas both markers were enriched in the nanovesicle fraction (Figure 3g). These results confirmed that apoptotic blebs and exosome-like nanovesicles produced by apoptotic EC represent two distinct entities, with different protein composition and function.
TCTP is a novel antiapoptotic component of the apoptotic secretome
We then sought to identify specific protein(s) involved in the antiapoptotic activity of exosome-like nanovesicles released by apoptotic EC. Three proteins known to be secreted through nanovesicles were identified concomitantly through functional (antiapoptotic) and comparative proteomics strategies (Table 1). Among these, TCTP appeared to be the most likely antiapoptotic candidate as it has known antiapoptotic activity in a number of cell types. Small interfering RNAs (siRNAs) were used to silence TCTP expression in EC, with the aim of reducing the release of TCTP-bearing nanovesicles by apoptotic EC. TCTP silencing reduced intracellular TCTP levels and inhibited TCTP release in nanovesicle extracts (Figure 4a and Supplementary Figure S3) but did not modulate the apoptosis of serum-starved EC (Figure 4b). TCTP-silenced EC or control EC were employed to condition equal volumes of serum-free media. Unfractionated SSC-Apo generated by TCTP-silenced EC (SSC siRNA TCTP) or its corresponding nanovesicle fraction failed to inhibit VSMC apoptosis, whereas control SSC-Apo (SSC siRNA Ctrl) or its corresponding nanovesicle fraction did so (Figure 4c). There was, however, no difference in the antiapoptotic activity of nanovesicle-free supernatants conditioned by serum-starved, TCTP-silenced and control EC (Figure 4c).
As ERK 1/2 activation is a characteristic feature of the antiapoptotic phenotype of neointimal cells, we evaluated whether TCTP induced ERK 1/2-dependent antiapoptotic pathways in VSMC. VSMC exposed to medium conditioned by siRNA TCTP (unfractionated and exosomal fraction) showed reduced ERK 1/2 phosphorylation in comparison with their respective controls (SSC siRNA Ctrl) (Figure 4c, lower panel). ERK 1/2 phosphorylation was similar in VSMC exposed to supernatants derived from media conditioned by TCTP-silenced or control EC. In addition, serum-starved VSMC exposed to recombinant TCTP (which included peptides identified by in-gel LC-MS/MS, Supplementary Figure S1d) manifested dose-dependent inhibition of apoptosis (Figure 4d) in association with increased ERK 1/2 activation (Figure 4e). The concentration of TCTP released by apoptotic EC in SSC-Apo was within the bioactive range (Supplementary Figure S1e). Inhibition of ERK 1/2 activation in VSMC with PD98059 blocked the antiapoptotic activity of recombinant TCTP (Figure 4f). Collectively, these results establish the importance of TCTP in the activation of an ERK 1/2-dependent antiapoptotic response in VSMC.
Increased TCTP export is characteristic of apoptotic cell death
To evaluate whether TCTP release by apoptotic cells was specific to EC, VSMC were serum starved in the presence of ZVAD-FMK or vehicle (DMSO). SS induced an apoptotic response in VSMC, which was blocked in the presence of ZVAD-FMK (Supplementary Figure S1f). Elevated TCTP levels were found in medium conditioned by apoptotic VSMC, compared with an equal volume of medium conditioned in the presence of ZVAD-FMK (Supplementary Information Figure S1f, lower panel). These data suggest that caspase activation favors TCTP export in different cell types.
As nutrient deprivation is a potent autophagic stimulus, we also considered the possibility that autophagy could contribute to TCTP export. EC exposed to rapamycin, a specific inhibitor of mammalian target of rapamycin, showed characteristic autophagic features as evaluated by acridine orange staining (Figure 5a), LC3 processing and electron microscopy (Figure 5c) in absence of apoptotic features as evaluated with HO-PI staining (Figure 5a) and PARP cleavage (Figure 5b). EC exposed to rapamycin failed to increase TCTP release (Figure 5d). Treatment with mitomycin C (MMC), another proapoptotic stimulus, increased the percentage of cells with chromatin condensation (Figure 5a), PARP cleavage (Figure 5b) and TCTP release (Figure 5d and Supplementary Figure S3). These results point to the activation of specific apoptosis-associated caspase(s) as a novel pathway regulating TCTP export.
Activated caspase-3 is a novel regulator of TCTP export
In serum-starved EC, TCTP export is initiated (Figure 6a) concomitantly with caspase-3 activation (Figure 1d). Biochemical pan-caspase inhibition or specific caspase-3 inhibition in serum-starved EC (preincubation with ZVAD-FMK or DEVD-FMK, respectively) concomitantly inhibited EC apoptosis (Figure 1g) and the release of antiapoptotic mediators active on VSMC (Figure 6b). In addition, TCTP levels were reduced in nanovesicle extracts from medium conditioned by serum-starved EC preincubated with DEVD-FMK, an irreversible caspase-3 inhibitor, compared with medium conditioned by apoptotic serum-starved EC (Figure 6c and Supplementary Figure S3).
To further address the importance of caspase-3 activation in TCTP export (and potential off-target effects of biochemical caspase inhibitors), siRNAs were used to silence caspase-3 expression in EC. Caspase-3 silencing significantly inhibited the apoptosis of serum-starved EC compared with EC transfected with control siRNAs (Figure 6d and e). In turn, VSMC exposed to medium conditioned by caspase-3-silenced EC (SSC siRNA C3) failed to mount an antiapoptotic response, whereas VSMC exposed to medium conditioned by control apoptotic EC (SSC siRNA Ctrl) developed an antiapoptotic phenotype (Figure 6f). TCTP levels were lower in unfractionated conditioned medium (Total) and in the nanovesicle fraction (Exo) of medium conditioned by caspase-3-silenced EC (SSC siRNA C3) compared with control apoptotic EC (SSC siRNA Ctrl) (Figure 6g and Supplementary Figure S3). Finally, we evaluated whether activated caspase-3 could directly cleave TCTP. Recombinant caspase-3 did not show any proteolytic activity toward recombinant TCTP in vitro but did cleave its known substrate PARP (Figure 6h). Also, total and nanovesicle fractions of SSC-Apo failed to show bands lower than the expected 23 kDa, ruling out a contribution of TCTP proteolysis. Collectively, these results demonstrate a key role for caspase-3 activation in the release of TCTP by apoptotic EC.
Discussion
Apoptotic cells actively release a finely regulated set of ‘come and eat-me’ and ‘stay-away’ paracrine signals aimed at coordinating the specific recruitment of mononuclear phagocytes.1, 2 Recent evidence indicates that the paracrine component of the apoptotic program is not limited to the regulation of leukocyte trafficking but also aims at preparing the local microenvironment for remodeling after cell deletion. The present work lends further support to this contention. Taking a multifaceted proteomics approach, we identified a set of 27 proteins released specifically by apoptotic EC (characterized by increased chromatin condensation and exclusion of propidium iodide (PI), loss of mitochondrial integrity and evidence of activated caspase-9 and -3) downstream of caspase activation. Several lines of evidence demonstrated that these proteins are not released as a consequence of cell membrane permeabilization. First, plasma membrane rupture, as evidenced by PI staining, is absent in serum-starved EC, and caspase inhibition does not impact cell membrane permeability. Second, LDH, a classical marker of cell membrane permeabilization, is not increased in medium conditioned by serum-starved apoptotic EC. Finally, the release of proteins by serum-starved EC is a targeted response, as Grp96 and tubulin are not secreted throughout SS, whereas TSG 101 and TCTP are released concomitantly with caspase activation.
Non-classical protein secretion pathways are, at least in part, responsible for the paracrine component of the apoptotic program in EC. Among the 27 proteins identified specifically in medium conditioned by apoptotic EC, more than half did not contain a secretion signal sequence. Also, irrespective of the presence of a secretion signal, more than a third corresponded to typical nanovesicle components. In recent years, the characterization of different types of microparticles and nanovesicles released by live cells has been under intense investigation. Unfortunately, there is yet no widely-accepted classification of the various categories of micro- and nanovesicles. Size, appearance under electron microscopy and intracellular origin are currently key features that differentiate various types of membrane vesicles. Exosomes are small, cup-shaped vesicles of 50–100 nm diameter.15, 21, 22, 23 Their precursors are intracellular vesicles packaged into MVB, which fuse with the plasma membrane, releasing exosomal vesicles into the extracellular milieu.15, 21, 22, 23 Exosome-like nanovesicles are somewhat smaller (20–50 nm), of irregular shape and probably stem also from endosomal compartments.15 Apoptotic blebs are bigger (50–500 nm), of heterogenous shapes and result from budding of the cell membrane.15, 24 The nanovesicles released by apoptotic EC share many characteristics with exosome-like nanovesicles and exosomes. Immunoblotting confirmed elevated levels of the exosomal markers, TCTP and TSG 101 in medium conditioned by apoptotic EC. Irregular-shaped nanovesicles of sizes within the range described for exosome-like nanovesicles were demonstrated by electron microscopy in medium conditioned by apoptotic EC. Immunogold labeling confirmed that TCTP was present at the surface of these nanovesicles and within MVB of apoptotic EC.
We, nonetheless, considered the possibility that nanovesicles released by apoptotic EC could represent small apoptotic blebs. Several lines of evidence suggest that TCTP-expressing nanovesicles differ from apoptotic blebs. First, TCTP and TSG 101 levels are high in nanovesicle fractions but undetectable in apoptotic bleb extracts. Second, histones, previously described as a specific component of apoptotic blebs15, 21 were not recovered with any of our proteomics strategies (data not shown), further confirming optimal depletion of apoptotic blebs before MS/MS analysis. Finally, exosome-like nanovesicles purified from medium conditioned by apoptotic EC trigger an antiapoptotic phenotype in VSMC, whereas apoptotic blebs purified from the same medium do not. These results indicate that over the course of apoptosis at least two functionally different types of vesicles are released: apoptotic blebs and nanovesicles. Whether the latter correspond to the enhanced production of exosome-like nanovesicles normally released by live EC or to a different nanovesicle type specific to the apoptotic program, sharing a common intracellular origin and at least some markers with exosome and exosome-like nanovesicles, will be the scope of future investigation.
Our work identifies activated caspase-3 as a novel regulator of TCTP export through the nanovesicle pathway. p53 is known to regulate TSAP-6 activity, which, in turn, controls exosome production and TCTP release.16, 17, 18 Here, increased release of nanovesicle constituents was identified by an unbiased proteomics strategy, where media conditioned by caspase-activated or -inactivated EC were compared. Caspase(s) inhibition with ZVAD-FMK impacts the execution phase of apoptosis but does not alter molecular events associated with apoptosis initiation, which includes similar intracellular p53 levels and mitochondrial permeabilization. Hence, p53 cannot be inferred as a regulator of TCTP export in our system. Caspase-3 biochemical inhibition or genetic silencing similarly prevents TCTP export, pointing to a pivotal role for caspase-3 in the release of TCTP-bearing nanovesicles by apoptotic cells.
Several lines of evidence indicate that TCTP plays a functional role in the antiapoptotic activity of nanovesicles released by apoptotic EC. VSMC exposed to TCTP-expressing nanovesicles show increased resistance to apoptosis and activation of ERK 1/2, therefore, recapitulating a neointimal phenotype.3, 9 TCTP silencing in EC blocks TCTP release and largely decreases both ERK 1/2 activation and resistance to apoptosis in VSMC exposed to nanovesicles produced by apoptotic EC. Finally, recombinant TCTP increases ERK 1/2 activation and inhibits VSMC apoptosis. TCTP is an evolutionarily conserved protein of crucial importance during development25 and for intracellular apoptosis inhibition.26, 27 The present work demonstrates that TCTP also displays significant extracellular antiapoptotic activity. These results are in keeping with recent investigations indicating that extracellular TCTP activates ERK 1/2 in basophils.
The present study highlights novel mechanisms of cross talk between dying cells and the local microenvironment. Apoptotic cells actively release apoptotic blebs and exosome-like nanovesicles. The latter, through an antiapoptotic activity on cells of importance in tissue and vascular repair, likely favor remodeling at sites of apoptotic cell deletion. However, a chronic increase in apoptosis could foster sustained activation of the paracrine program, resulting in maladaptive remodeling.
Materials and Methods
Cell culture and generation of conditioned media
HUVEC (Clonetics, San Diego, CA, USA) were grown in microvascular EC medium (Clonetics) and used at passages 2–5. WI-38 human fibroblasts (ATCC, Rockville, MD, USA) were grown in FBM (Cambrex, Walkersville, MD, USA) with 10% inactivated FBS (Medicorp, Montréal, Qc, Canada) and employed at passages 2–17. A7R5 cells (VSMC), a clonal rat smooth muscle cell line (ATCC), were cultured in DMEM/F12 with 10% FBS. Serum-free media, conditioned by apoptotic or caspase-inhibited EC, were obtained as described previously.3, 4, 5, 6, 7, 8 Equal EC numbers (2.5 × 104 cells/cm2) were preincubated for 2 h in normal medium containing either DMSO (vehicle) or ZVAD-FMK (100 μM) or DEVD-FMK (100 μM) (R&D Systems, Minneapolis, MN, USA) for caspase(s) inhibition. Then, the culture medium was changed for serum-free medium RPMI (Gibco, Burlington, Ontario, Canada) and EC were serum starved for 4 h.
Characterization of the secretome produced by apoptotic EC
We adopted two comparative proteomics approaches to identify the secretome released by apoptotic EC: 2D-LC-MS/MS and SDS-PAGE LC-MS/MS.14 Serum-free media (0.16 ml/cm2) conditioned by apoptotic (SSC-Apo) and non-apoptotic EC preincubated with ZVAD-FMK (SSC-No-Apo) were centrifuged sequentially at 1200 × g and 50 000 × g to eliminate cell debris and apoptotic blebs, and depletion was confirmed by flow cytometry (FACScan equipped with CellFit software, Becton-Dickinson, San José, CA, USA) in FL1 and FL2 channels. We also performed a functional analysis of SSC-Apo. A total of 750 ml of medium conditioned by apoptotic EC was fractionated by FPLC, and each fraction was tested for antiapoptotic activity on VSMC.3 The antiapoptotic fraction was resolved by SDS-PAGE, and the bands were sequenced with LC-MS/MS.
For 2D-LC-MS/MS analysis, 40 ml of conditioned media cleared of cell debris and apoptotic blebs were concentrated (0.5 mg of proteins) and solubilized in 100 μl of 40 mM Tris-HCl, pH 8.0, 7.5 M urea, 2.0 M thiourea, reduced in the presence of 6 mM DTT, alkylated with 15 mM iodoacetamide and digested overnight with trypsin (Promega, Madison, WI, USA, sequencing grade, estimated trypsin/protein ratio 1 : 100). The tryptic peptides were resuspended in 55% acetonitrile, 25% dimethylformamide and labeled with pentafluorophenyl-4-anilino-4-oxobutanoate-do or pentafluorophenyl-4-anilino-4-oxobutanoate-d5. Labeled samples were combined, desalted, evaporated to dryness, resuspended in 10% acetonitrile, containing 10 mM ammonium acetate, pH 7.0, and analyzed by weak anion exchange chromatography in a PolyWAX column (100 × 1 mm, 5 μm, 300 Å; PolyLC, Columbia, MO, USA) connected to an Agilent 1100 Series LC system (Santa Clara, CA, USA). Peptides were eluted by a gradient of 0–1 M NaCl in 10 mM ammonium acetate, pH 6.0, containing 10% acetonitrile, at a flow rate of 20 μl/min. A total of 36 fractions of 80 μl were collected and acidified with formic acid. A total of 30 μl from each fraction were analyzed by LC-MS/MS.
SDS-PAGE LC-MS/MS analysis was performed essentially as outlined elsewhere14. Proteins (125 μg) were solubilized in 4 × Laemmli buffer (62.5 mM Tris-HCl, pH 6.8, 20% glycerol, 2% SDS, 0.5% (w/v) bromophenol blue), reduced in the presence of 4 mM DTT for 1 h at room temperature and then alkylated with 10 mM phenylmaleimide for 1 h at room temperature. A total of 125 μg of total protein from each sample were separated by SDS-PAGE on 15% acrylamide gel, which was stained with Coomassie blue. Each lane was cut into 20 slices and treated with trypsin (Promega). Tryptic peptides were extracted with 60% acetonitrile and 0.1% formic acid, evaporated to dryness and resuspended in 25 μl of 3% acetonitrile and 0.1% formic acid.
Peptide digests were analyzed in duplicate by LC-MS/MS consisting of an Agilent 1100 Series nanoflow liquid chromatography system and a 1100 Series LC/MSD-Trap-SL ion trap mass spectrometer (Agilent Technologies). The peptides were enriched in a Zorbax 300SB-C18 trap column (5 μm, 5 × 0.3 mm) and separated by reverse phase chromatography in a Zorbax 300SB-C18 analytical column (Mississauga, Ontario, Canada) (3.5 μm, 150 × 0.075 mm) with a gradient of 5–90% acetonitrile in 0.1% formic acid at a flow rate of 300 nl/min. The acquisition parameters were as follows: (a) positive mode, (b) scan range from 400 to 2200 Da, (c) ‘trap drive’ of 90, (d) maximum 3 MS/MS per cycle, (e) preferred charge state of +2, (f) active exclusion after two spectra for 1 min and (g) scan speed of 13 000 m/z/sec. Spectra were recorded in profile mode.
The mass spectra were interpreted and quantified by Spectrum Mill software (Rev. A.03.02.060a, Agilent Technologies). Using a ‘Data Extractor’ module of the program, the MS/MS spectra were: (a) converted to a centroid mode based on the area in the top 50% of peak intensity, (b) merged by similarity (for two spectra to be merged, at least 25 out of their 50 most intensive peaks had to match and the matching peaks had to represent >70% of the total spectral intensity) within a time window of ±40 s and m/z window ±1.2 Da, and (c) filtered by quality (precursor signal to noise ratio >25, sequence tag length >1). For every spectrum, MS intensity was calculated as the area under the extracted chromatogram of ion intensity versus retention time (EIC) employing the same parameters as for merging. ‘MS/MS search’ was performed for the 25 most intensive peaks in every spectrum with the human UniProt database (7 September, 2006 release: ftp://ftp.expasy.org).
Immunoblotting and reagents
Protein extracts were separated on 12% SDS-PAGE, as described previously,3, 4, 5, 6, 7, 8 and probed with monoclonal antibodies against: procaspase-3 (Bio Vision Research Products, Mountain View, CA, USA), activated caspase-3 (Cell Signalling Technology, Pickering, Ontario, Canada), activated caspase-9 (Calbiochem, San Diego, CA, USA), TCTP (Santa Cruz Biotechnology, Santa Cruz, CA, USA), p53 (Santa Cruz Biotechnology), actin (Cedarlane, Burlington, Ontario, Canada), TSG 101 (Abcam, Cambridge, MA, USA), Grp96 (Abcam), tubulin (Oncogene, Boston, MA, USA), phospho-ERK 1/2 (New England Biolabs, Pickering, Ontario, Canada), ERK2 (Santa Cruz Biotechnology), PARP (Cell Signaling) and LC-3 (Abnova Antibody Innovation, Walnut, CA, USA). Protein extracts from the supernatants were TCA precipitated 9 : 1, washed with cold acetone and solubilized in sample buffer. MMC, rapamycin, TCEP (tris (2-carboxyethyl) phosphine) and recombinant PARP were from Sigma (Oakville, Ontario, Canada). Recombinant GST-TCTP and GST were obtained from Abnova Antibody Innovation. LEHD-FMK was from R&D Systems and PD98059 from Calbiochem. Activated recombinant caspase-3 was obtained from Enzo Life Sciences (Plymouth Meeting, PA, USA).
Fluorescence microscopy for quantization of cells with chromatin condensation and cell membrane permeabilization
Fluorescence microscopy of unfixed/unpermeabilized adherent cells stained with Hoechst 33342 (2′-(4-ethoxyphenyl)-5-(4-methyl-1-piperazinyl)-2.5′-bi-1H-benzimidazole) (HO) and PI was undertaken as described previously.3, 4, 5 In brief, cells were grown to confluence in 24-well polycarbonate culture plates (Becton-Dickinson). HO (1 μg/ml) was added for 10 min at 37 °C, and the cells were washed with PBS. PI was added to a final concentration of 5 μg/ml immediately before fluorescence microscopy analysis (excitation filter l=360–425 nm). The percentages of normal, apoptotic and necrotic cells adherent to the dishes were estimated by an investigator blinded to the experimental conditions. Apoptotic cells will show increased HO fluorescence in absence of PI positivity. Secondary and primary necrotic cells show PI positivity.
Mitochondrial permeability assessment
Loss of mitochondrial permeability of EC was assessed by JC-1 (Molecular Probes, Invitrogen, Burlington, Ontario, Canada) staining and flow cytometry.28 Cells were incubated with JC-1 (10 μg/ml) for 15 min, harvested by trypsinization and washed twice with cold PBS. Loss of mitochondrial permeability is indicated by shifting in fluorescence emission from green to red, which was evaluated by flow cytometry (Coulter EPICS XL-MLC flow cytometer, Mississauga, Ontario, Canada) in FL1 and FL2 channels. A total of 10 000 events per sample were acquired and the results expressed as fold increase of EC, with loss of mitochondrial permeability relative to control EC exposed to normal medium for 4 h (percentage of experimental cells with red fluorescence/percentage of control cells with red fluorescence).
LDH release assay
LDH release was analyzed by Cyto Tox 96 non-radioactive cytotoxicity assay (Promega), as described by the manufacturer.The results are expressed as the percentage of absorbance at 490 nm of experimental conditions versus absorbance at 490 nm of the positive control for necrosis (heating).
Acridine orange staining
Acidic vesicular organelles, which correlate with autophagic activity, were assessed as described previously.29 In acridine orange-stained cells, the cytoplasm and nucleolus fluoresce bright green and dim red, whereas acidic compartments fluoresce bright red, evaluated by fluorescence microscopy (excitation filter 1=525–625 nm).
Purification of nanovesicles by differential centrifugation
Nanovesicles were prepared from HUVEC and VSMC supernatants by differential centrifugation, as outlined elsewhere30 with some modifications. Conditioned media were centrifuged sequentially at 1200 × g for 20 min to remove cell debris, 50 000 × g for 15 min to eliminate apoptotic blebs and 100 000 × g for 18 h (Beckman SW-41 Ti rotor, Mississauga, Ontario, Canada) to purify the exosomal fraction. For western blot analysis, exosomes were harvested in phosphate buffer (0.1 M), precipitated with TCA 9 : 1, washed with cold acetone and solubilized in SDS-PAGE sample buffer (Bio Rad, Mississauga, Ontario, Canada).
Electron microscopy
For immunogold labeling, nanovesicles isolated as above were adsorbed on parlodium-carbon-coated electron microscopy grids and fixed with 4% paraformaldehyde. After washing, the grids were floated on ovalbumin 1% for 5 min and anti-TCTP antibody (1 : 20 dilution) for 2 h at room temperature, washed with PBS, transferred to protein A-gold (10 nm), washed with PBS and MilliQ water (Billerica, MA, USA), and dried. Uranyl acetate and phosphotungstic acid-negative staining was undertaken, and images were recorded with a Phillips 410 transmission electron microscope (Montréal, Québec, Canada). HUVEC were fixed with paraformaldehyde lysine periodate, dehydrated in increasing methanol solutions and embedded in Lowicryl K4M (Canemco, Lakefield, Qc, Canada) at −20 °C. For immunocytochemical detection of TCTP, ultrathin sections were incubated in saturated sodium metaperiodate for 8 min, washed with MilliQ water, quenched with ovalbumin 1% and labeled with anti-TCTP (1 : 10 dilution) for 4 h at room temperature, followed by protein A-gold (5 or 10 nm). The tissues were stained with uranyl acetate and lead citrate.31 For quantification of volume density of MVB and autophagosomes, EC were fixed in glutaraldehyde, postfixed in osmium tetroxyde and embedded in Epon. Electron micrograph fields of the cell cytoplasm were recorded at × 7000 and enlarged at × 21000. The volume density of the MVB and the autophagosomes was evaluated in relation to the cell cytoplasm (nuclei were not included in the evaluation) by direct planimetry using the Zeiss Videopan software (Toronto, Ontario, Canada) (MVB area/cell area μm2).
Caspase-3 and TCTP silencing
EC were grown in 6- and 24-well plates until 90% confluence per well. Transfection was performed with Oligofectamine (Invitrogen Life Technologies, Burlington, Ontario, Canada) using ON-TARGET plus SMART pool (Dharmacon, Nepean, Ontario, Canada) for caspase-3, TCTP and control siRNAs. SiRNAs were used at a final concentration of 50 nM (caspase-3) and 200 nM (TCTP) of annealed oligo for 16 h, changed in normal medium for 72 h (caspase-3) and 48 h (TCTP) and serum starved for 4 h.
Statistical analysis
The data, expressed as mean±S.E.M., were analyzed by Student's T-test (with Bonferroni correction when appropriate) or ANOVA, as appropriate.
Abbreviations
- 2D-LC-MS/MS:
-
two-dimensional liquid chromatography and tandem mass spectrometry
- CTGF:
-
connective tissue growth factor
- DMSO:
-
dimethylsulfoxide
- EC:
-
endothelial cells
- ERK 1/2:
-
extracellular signal-regulated kinases 1/2
- FPLC:
-
fast protein liquid chromatography
- HO:
-
Hoechst 33342 (2′-(4-ethoxyphenyl)-5-(4-methyl-1-piperazinyl)-2.5′-bi-1H-benzimidazole)
- HUVEC:
-
human umbilical vascular endothelial cells
- LDH:
-
lactate dehydrogenase
- LG3:
-
C-terminal fragment of perlecan
- MMC:
-
mitomycin C
- MVB:
-
multivesicular bodies
- PARP:
-
poly(ADP-ribose) polymerase
- PI:
-
propidium iodide
- SDS-PAGE:
-
sodium dodecyl sulfate-polyacrylamide gel electrophoresis
- siRNAs:
-
small interfering RNAs
- SN:
-
exosome-free supernatant
- SS:
-
serum starvation
- SSC:
-
serum-free media conditioned by endothelial cells
- TCTP:
-
translationally-controlled tumor protein
- TSG 101:
-
tumor susceptibility gene 101
- VSMC:
-
vascular smooth muscle cells
- LC3:
-
microtubule-associated proteins 1A and 1B, light chain 3
- mTOR:
-
mammalian target of rapamycin
References
Lauber K, Bohn E, Krober SM, Xiao YJ, Blumenthal SG, Lindemann RK et al. Apoptotic cells induce migration of phagocytes via caspase-3-mediated release of a lipid attraction signal. Cell 2003; 113: 717–730.
Bournazou I, Pound JD, Duffin R, Bournazos S, Melville LA, Brown SB et al. Apoptotic human cells inhibit migration of granulocytes via release of lactoferrin. J Clin Invest 2009; 119: 20–32.
Raymond MA, Desormeaux A, Laplante P, Vigneault N, Filep JG, Landry K et al. Apoptosis of endothelial cells triggers a caspase-dependent anti-apoptotic paracrine loop active on VSMC. Faseb J 2004; 18: 705–707.
Laplante P, Raymond MA, Gagnon G, Vigneault N, Sasseville AM, Langelier Y et al. Novel fibrogenic pathways are activated in response to endothelial apoptosis: implications in the pathophysiology of systemic sclerosis. J Immunol 2005; 174: 5740–5749.
Laplante P, Raymond MA, Labelle A, Abe J, Iozzo RV, Hebert MJ . Perlecan proteolysis induces an alpha2beta1 integrin- and Src family kinase-dependent anti-apoptotic pathway in fibroblasts in the absence of focal adhesion kinase activation. J Biol Chem 2006; 281: 30383–30392.
Cailhier JF, Sirois I, Laplante P, Lepage S, Raymond MA, Brassard N et al. Caspase-3 activation triggers extracellular cathepsin L release and endorepellin proteolysis. J Biol Chem 2008; 283: 27220–27229.
Soulez M, Sirois I, Brassard N, Raymond MA, Nicodeme F, Noiseux N et al. Epidermal growth factor and perlecan fragments produced by apoptotic endothelial cells co-ordinately activate ERK1/2-dependent antiapoptotic pathways in mesenchymal stem cells. Stem Cells 2010; 28: 810–820.
Laplante P, Sirois I, Raymond MA, Kokta V, Beliveau A, Prat A et al. Caspase-3-mediated secretion of connective tissue growth factor by apoptotic endothelial cells promotes fibrosis. Cell Death Differ 2010; 17: 291–303.
Cailhier JF, Laplante P, Hebert MJ . Endothelial apoptosis and chronic transplant vasculopathy: recent results, novel mechanisms. Am J Transplant 2006; 6: 247–253.
Cornell LD, Smith RN, Colvin RB . Kidney transplantation: mechanisms of rejection and acceptance. Annu Rev Pathol 2008; 3: 189–220.
Pollman MJ, Hall JL, Mann MJ, Zhang L, Gibbons GH . Inhibition of neointimal cell bcl-x expression induces apoptosis and regression of vascular disease. Nat Med 1998; 4: 222–227.
Gennaro G, Menard C, Michaud SE, Deblois D, Rivard A . Inhibition of vascular smooth muscle cell proliferation and neointimal formation in injured arteries by a novel, oral mitogen-activated protein kinase/extracellular signal-regulated kinase inhibitor. Circulation 2004; 110: 3367–3371.
Hirata A, Igarashi M, Yamaguchi H, Suwabe A, Daimon M, Kato T et al. Nifedipine suppresses neointimal thickening by its inhibitory effect on vascular smooth muscle cell growth via a MEK-ERK pathway coupling with Pyk2. Br J Pharmacol 2000; 131: 1521–1530.
Pshezhetsky AV, Fedjaev M, Ashmarina L, Mazur A, Budman L, Sinnett D et al. Subcellular proteomics of cell differentiation: quantitative analysis of the plasma membrane proteome of Caco-2 cells. Proteomics 2007; 7: 2201–2215.
Thery C, Ostrowski M, Segura E . Membrane vesicles as conveyors of immune responses. Nat Rev Immunol 2009; 9: 581–593.
Amzallag N, Passer BJ, Allanic D, Segura E, Thery C, Goud B et al. TSAP6 facilitates the secretion of translationally controlled tumor protein/histamine-releasing factor via a nonclassical pathway. J Biol Chem 2004; 279: 46104–46112.
Yu X, Harris SL, Levine AJ . The regulation of exosome secretion: a novel function of the p53 protein. Cancer Res 2006; 66: 4795–4801.
Lespagnol A, Duflaut D, Beekman C, Blanc L, Fiucci G, Marine JC et al. Exosome secretion, including the DNA damage-induced p53-dependent secretory pathway, is severely compromised in TSAP6/Steap3-null mice. Cell Death Differ 2008; 15: 1723–1733.
Yoon T, Jung J, Kim M, Lee KM, Choi EC, Lee K . Identification of the self-interaction of rat TCTP/IgE-dependent histamine-releasing factor using yeast two-hybrid system. Arch Biochem Biophys 2000; 384: 379–382.
Kim M, Min HJ, Won HY, Park H, Lee JC, Park HW et al. Dimerization of translationally controlled tumor protein is essential for its cytokine-like activity. PLoS ONE 2009; 4: e6464.
Thery C, Boussac M, Veron P, Ricciardi-Castagnoli P, Raposo G, Garin J et al. Proteomic analysis of dendritic cell-derived exosomes: a secreted subcellular compartment distinct from apoptotic vesicles. J Immunol 2001; 166: 7309–7318.
Thery C, Zitvogel L, Amigorena S . Exosomes: composition, biogenesis and function. Nat Rev Immunol 2002; 2: 569–579.
Li XB, Zhang ZR, Schluesener HJ, Xu SQ . Role of exosomes in immune regulation. J Cell Mol Med 2006; 10: 364–375.
Kroemer G, Galluzzi L, Vandenabeele P, Abrams J, Alnemri ES, Baehrecke EH et al. Classification of cell death: recommendations of the Nomenclature Committee on Cell Death 2009. Cell Death Differ 2009; 16: 3–11.
Chen SH, Wu PS, Chou CH, Yan YT, Liu H, Weng SY et al. A knockout mouse approach reveals that TCTP functions as an essential factor for cell proliferation and survival in a tissue- or cell type-specific manner. Mol Biol Cell 2007; 18: 2525–2532.
Telerman A, Amson R . The molecular programme of tumour reversion: the steps beyond malignant transformation. Nat Rev Cancer 2009; 9: 206–216.
Vonakis BM, Macglashan Jr DW, Vilarino N, Langdon JM, Scott RS, MacDonald SM . Distinct characteristics of signal transduction events by histamine-releasing factor/translationally controlled tumor protein (HRF/TCTP)-induced priming and activation of human basophils. Blood 2008; 111: 1789–1796.
Paquet C, Sane AT, Beauchemin M, Bertrand R . Caspase- and mitochondrial dysfunction-dependent mechanisms of lysosomal leakage and cathepsin B activation in DNA damage-induced apoptosis. Leukemia 2005; 19: 784–791.
Takeuchi H, Kanzawa T, Kondo Y, Kondo S . Inhibition of platelet-derived growth factor signalling induces autophagy in malignant glioma cells. Br J Cancer 2004; 90: 1069–1075.
Raposo G, Nijman HW, Stoorvogel W, Liejendekker R, Harding CV, Melief CJ et al. B lymphocytes secrete antigen-presenting vesicles. J Exp Med 1996; 183: 1161–1172.
Bendayan M . Tech.Sight. Worth its weight in gold. Science 2001; 291: 1363–1365.
Pisitkun T, Shen RF, Knepper MA . Identification and proteomic profiling of exosomes in human urine. Proc Natl Acad Sci USA 2004; 101: 13368–13373.
Gutwein P, Stoeck A, Riedle S, Gast D, Runz S, Condon TP et al. Cleavage of L1 in exosomes and apoptotic membrane vesicles released from ovarian carcinoma cells. Clin Cancer Res 2005; 11: 2492–2501.
Wubbolts R, Leckie RS, Veenhuizen PT, Schwarzmann G, Mobius W, Hoernschemeyer J et al. Proteomic and biochemical analyses of human B cell-derived exosomes. Potential implications for their function and multivesicular body formation. J Biol Chem 2003; 278: 10963–10972.
Aronov S, Gelin-Licht R, Zipor G, Haim L, Safran E, Gerst JE . mRNAs encoding polarity and exocytosis factors are cotransported with the cortical endoplasmic reticulum to the incipient bud in Saccharomyces cerevisiae. Mol Cell Biol 2007; 27: 3441–3455.
Nguyen NV, Gleeson PA, Courtois-Coutry N, Caplan MJ, Van Driel IR . Gastric parietal cell acid secretion in mice can be regulated independently of H/K ATPase endocytosis. Gastroenterology 2004; 127: 145–154.
Wang P, Tortorella M, England K, Malfait AM, Thomas G, Arner EC et al. Proprotein convertase furin interacts with and cleaves pro-ADAMTS4 (Aggrecanase-1) in the trans-Golgi network. J Biol Chem 2004; 279: 15434–15440.
Emeis JJ, van den Eijnden-Schrauwen Y, van den Hoogen CM, de Priester W, Westmuckett A, Lupu F . An endothelial storage granule for tissue-type plasminogen activator. J Cell Biol 1997; 139: 245–256.
van Niel G, Raposo G, Candalh C, Boussac M, Hershberg R, Cerf-Bensussan N et al. Intestinal epithelial cells secrete exosome-like vesicles. Gastroenterology 2001; 121: 337–349.
Segura E, Amigorena S, Thery C . Mature dendritic cells secrete exosomes with strong ability to induce antigen-specific effector immune responses. Blood Cells Mol Dis 2005; 35: 89–93.
Acknowledgements
This work was supported by research grants from the Canadian Institutes of Health Research to MJH (MOP-15447) and the Canadian Institutes of Health Research to AVP (MOP-66980). MJH is the holder of the Shire Chair in Nephrology, Transplantation and Renal Regeneration of the University of Montreal. IS is the recipient of a training fellowship from the Canadian Institutes of Health Research. JFC is an FRSQ scholar. We thank the J-L Lévesque Foundation for renewed support, Nicolas Parent for help with JC-1 staining assay and D. Gingras for processing cells for electron microscopy.
Author information
Authors and Affiliations
Corresponding author
Ethics declarations
Competing interests
The authors declare no conflict of interest.
Additional information
Edited by P Vandenabeele
Supplementary Information accompanies the paper on Cell Death and Differentiation website
Rights and permissions
About this article
Cite this article
Sirois, I., Raymond, MA., Brassard, N. et al. Caspase-3-dependent export of TCTP: a novel pathway for antiapoptotic intercellular communication. Cell Death Differ 18, 549–562 (2011). https://doi.org/10.1038/cdd.2010.126
Received:
Revised:
Accepted:
Published:
Issue Date:
DOI: https://doi.org/10.1038/cdd.2010.126
Keywords
This article is cited by
-
Exosomes derived from programmed cell death: mechanism and biological significance
Cell Communication and Signaling (2024)
-
Advances in biological functions and applications of apoptotic vesicles
Cell Communication and Signaling (2023)
-
Apoptotic exosome-like vesicles transfer specific and functional mRNAs to endothelial cells by phosphatidylserine-dependent macropinocytosis
Cell Death & Disease (2023)
-
Apoptotic exosome-like vesicles regulate endothelial gene expression, inflammatory signaling, and function through the NF-κB signaling pathway
Scientific Reports (2020)
-
Apoptotic cell-derived exosomes: messages from dying cells
Experimental & Molecular Medicine (2020)