Next Article in Journal
S-Adenosine Methionine (SAMe) and Valproic Acid (VPA) as Epigenetic Modulators: Special Emphasis on their Interactions Affecting Nervous Tissue during Pregnancy
Next Article in Special Issue
Involvement of POLA2 in Double Strand Break Repair and Genotoxic Stress
Previous Article in Journal
An Evaluation of the In Vitro Roles and Mechanisms of Silibinin in Reducing Pyrazinamide- and Isoniazid-Induced Hepatocellular Damage
Previous Article in Special Issue
Norepinephrine-Induced DNA Damage in Ovarian Cancer Cells
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
IJMS
Volume 21
Issue 10
10.3390/ijms21103720
ijms-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Article

DNA Damage Regulates Senescence-Associated Extracellular Vesicle Release via the Ceramide Pathway to Prevent Excessive Inflammatory Responses

by
Kazuhiro Hitomi
1,2,†,
Ryo Okada
1,†,
Tze Mun Loo
1,
Kenichi Miyata
1,
Asako J. Nakamura
2 and
Akiko Takahashi
1,3,4,*
1
Project for Cellular Senescence, The Cancer Institute, Japanese Foundation for Cancer Research, Koto-ku, Tokyo 135-8550, Japan
2
Graduate School of Science and Engineering, Ibaraki University, Mito, Ibaraki 310-8512, Japan
3
Precursory Research for Embryonic Science and Technology (PRESTO), Japan Science and Technology Agency (JST), Kawaguchi, Saitama 332-0012, Japan
4
Advanced Research & Development Programs for Medical Innovation (PRIME), Japan Agency for Medical Research and Development (AMED), Chiyoda-ku, Tokyo 104-0004, Japan
*
Author to whom correspondence should be addressed.
†
These authors contributed equally to this work.
Int. J. Mol. Sci. 2020, 21(10), 3720; https://doi.org/10.3390/ijms21103720
Submission received: 29 April 2020 / Revised: 15 May 2020 / Accepted: 19 May 2020 / Published: 25 May 2020
(This article belongs to the Special Issue Recognition of DNA Lesions)
Browse Figures
Review Reports Versions Notes

Abstract

:
DNA damage, caused by various oncogenic stresses, can induce cell death or cellular senescence as an important tumor suppressor mechanism. Senescent cells display the features of a senescence-associated secretory phenotype (SASP), secreting inflammatory proteins into surrounding tissues, and contributing to various age-related pathologies. In addition to this inflammatory protein secretion, the release of extracellular vesicles (EVs) is also upregulated in senescent cells. However, the molecular mechanism underlying this phenomenon remains unclear. Here, we show that DNA damage activates the ceramide synthetic pathway, via the downregulation of sphingomyelin synthase 2 (SMS2) and the upregulation of neutral sphingomyelinase 2 (nSMase2), leading to an increase in senescence-associated EV (SA-EV) biogenesis. The EV biogenesis pathway, together with the autophagy-mediated degradation pathway, functions to block apoptosis by removing cytoplasmic DNA fragments derived from chromosomal DNA or bacterial infections. Our data suggest that this SA-EV pathway may play a prominent role in cellular homeostasis, particularly in senescent cells. In summary, DNA damage provokes SA-EV release by activating the ceramide pathway to protect cells from excessive inflammatory responses.

Graphical Abstract

1. Introduction

DNA damage can have numerous chemical and biological effects on cellular function and may induce apoptotic cell death or cellular senescence in healthy cells [1,2]. Cellular senescence is an important tumor suppression mechanism. It acts as a barrier against various oncogenic stresses, such as telomere shortening, oncogene activation, irradiation, or stimuli that damage DNA [3,4,5]. These stressors activate p53, followed by an increase in p21WAF1/CIP1 and/or p16INK4a expression. These are cyclin-dependent kinase inhibitors that promote the activation of retinoblastoma protein (RB), resulting in irreversible cell cycle arrest in normal cells [6,7,8]. Based on in vivo imaging analysis, using p21WAF1/CIP1 or p16INK4a transgenic mice, we found that senescent cells accumulated throughout their bodies during the aging process [9,10,11]. Recently, it was shown that senescent cells increase the expression of inflammatory genes and produce various secretory proteins, such as cytokines, chemokines, growth factors, and matrix metalloproteinases [12,13]. This phenotype is referred to as the senescence-associated secretory phenotype (SASP) and is known to cause chronic inflammation in surrounding tissues [5,14,15]. SASP is associated with multiple age-related pathologies, such as cancer [16]. SASP-factor gene expression is transcriptionally regulated by nuclear factor κB (NF-κB) or CCAAT/enhancer-binding protein β (C/EBP-β) in senescent cells [17]. In addition, DNA damage signaling is important for SASP-factor gene expression, both through the epigenetic modification of chromatin [18] and by activation of the innate immune response via the cyclic GMP-AMP synthase (cGAS)-stimulator of interferon genes (STING) pathway after chromosomal DNA fragments accumulate in the cytoplasm [19,20,21,22,23].
Notably, recent evidence has shown that senescent cells secrete not only inflammatory proteins, but also small extracellular vesicles (EVs) [24,25,26], which contain various cellular components, such as proteins, lipids, and nucleic acids, and thereby play a role in cell-to-cell communication [27,28,29]. Small EVs, released from senescent cells, contribute to cancer cell proliferation and the induction of cellular senescence in neighboring cells, as so-called SASP factors [16,25,30,31]. In addition, we previously reported that small EV secretion is an essential defense mechanism for avoiding the aberrant activation of DNA damage responses in normal cells and for maintaining cellular homeostasis by the excretion of toxic self-DNA or viral DNA into the extracellular space [24]. However, the detailed molecular mechanism of EV biogenesis, triggered by DNA damage signaling in senescent cells, has yet to be elucidated fully. In this study, we demonstrated that DNA damage promotes activation of the ceramide pathway and increases the release of small EVs. Furthermore, this pathway, in conjunction with autophagy, prevents excessive inflammatory responses against bacterial infection.

2. Results

2.1. DNA Damage Induces Small EV Secretion from Normal Human Fibroblasts and Epithelial Cells

To evaluate the effect of DNA damage on small EV secretion from normal human diploid fibroblasts (HDFs), TIG-3 cells were treated with a DNA-damaging agent, doxorubicin (DXR). Treatment with DXR increased the signs of the DNA damage response (DDR) in a dose-dependent manner, as judged by DNA damage foci (the phosphorylation of H2AX and the consensus target sequences of ATM/ATR) (Figure 1A). Consistent with several previous reports [24,26,32,33], nanoparticle tracking analysis (NTA) revealed that an increase in small EV secretion was concomitant with the level of DNA damage (Figure 1B). Since DNA damage is known to cause cellular senescence in normal cells, we investigated the molecular mechanism of small EV secretion, induced by DNA damage, using both young and senescent HDFs. We confirmed the induction of cellular senescence by RT-qPCR analysis of p16INK4a, a well-established marker of cellular senescence, in DNA damage- or oncogene (HRasV12)-induced senescent cells (Figure 1C) [6,7,8]. Recent studies have shown that there are many factors involved in regulating the biogenesis and release of small EVs, such as the ceramide pathway, ESCRT (endosomal sorting complexes required for transport), and Rab-family small GTPases [34,35,36,37]. Of these, we focused on lipid-related proteins because the sphingolipid pathway might modulate the budding of intraluminal membrane vesicles (ILVs) into multivesicular bodies (MVBs) and regulate small EV biogenesis [34,38]. Here, we revealed that the gene expression of sphingomyelin synthase 2 (SMS2) was downregulated significantly while, conversely, that of neutral sphingomyelinase 2 (nSMase2) was upregulated in both types of senescent cells (Figure 1C,D). Sphingomyelinase activation and sphingomyelin synthase inhibition result in ceramide production, which is related to the promotion of small EV biogenesis and increased EV release from several cell types [34,38,39,40,41]. Therefore, we speculated that activating the ceramide synthetic pathway after DNA damage might be important for small EV release from both healthy control and senescent cells. To confirm our findings in another cell line, human retinal pigment epithelial cells (RPE-1 cells) were also treated with DXR to induce cellular senescence. In accordance with DDR induction and p16INK4a upregulation (Figure 1E, F), the gene expression of both SMS2 and nSMase2 in the epithelial cells was changed in a similar manner to that seen in senescent HDFs (Figure 1F,G). Next, small EVs were subject to NTA, demonstrating that the release of small EVs also increased in senescent epithelial cells, compared with their release in healthy control cells (Figure 1H). In addition, transmission electron microscopy analysis using immuno-gold labelling for CD63, a well-known exosome marker [42], showed that these cells were secreting exosomes among the small EVs (Figure 1I). These data indicated that DNA damage activates the ceramide synthetic pathway in both HDFs and epithelial cells.

2.2. Activation of the Ceramide Synthetic Pathway Promotes Small EV Release from Cells

The expression levels of both SMS2 and nSMase2 changed in senescent cells; therefore we investigated these proteins’ roles in small EV release from HDFs. First, we used small interfering RNA (siRNA) to knock-down SMS2 [43], causing a significant induction of small EV secretion from HDFs, as determined by NTA (Figure 2A–C). Conversely, SMS2 overexpression reduced the level of small EV secretion after DXR treatment (Figure 2D,E). Second, nSMase2 depletion substantially reduced small EV secretion (Figure 2F–H) [38]. Importantly, inhibiting small EV secretion provoked the aberrant activation of DNA damage signaling in normal HDFs, as previously reported (Figure 2I) [24]. Furthermore, nSMase2 overexpression resulted in remarkably enhanced small EV release (Figure 2J,K). Taken together, these results revealed that activating the ceramide synthetic pathway promotes the release of small EV from cells.

2.3. Small EV Release Via the Ceramide Pathway Prevents DNA Damage Accumulation in Mice

In order to examine the effect of the ceramide synthetic pathway on both small EV release and tissue homeostasis in vivo, we used a chemical inhibitor of nSMase, spiroepoxide, which blocks small EV production in human cells [24,41]. We also observed the same effects in mouse embryonic fibroblasts (MEFs) by spiroepoxide treatment (Figure 3A). It is notable that inhibiting the ceramide pathway clearly induced cell cycle arrest and DNA damage accumulation in MEFs (Figure 3B,C). Next, we treated mice with spiroepoxide for 14 days. As expected, the inhibitor treatment reduced small EV release from the small intestine and accumulated DNA damage in mice tissues (Figure 3D,E). Collectively, our data strongly suggested that the ceramide pathway plays a crucial role in vivo in releasing small EVs and maintaining tissue homeostasis to avoid DNA damage accumulation.

2.4. The Autophagy Pathway Prevents Accumulation of Chromosomal DNA Fragments in the Cytoplasm to Block SASP-Factor Gene Expression in Accompany with Small EV Release

The accumulation of chromosomal DNA fragments in the cytoplasm promotes aberrant activation of the DNA-sensing pathway and causes global SASP-factor gene expression, both of which are associated with chronic inflammation and various age-related pathologies [15,16]. Cytoplasmic DNA fragments are so dangerous that normal cells prevent their accumulation via several degradation mechanisms, such as cytoplasmic DNases and the autophagy pathway [44]. We previously reported that the expression of the cytoplasmic DNases, DNase2 and TREX1, is regulated by E2F transcription factors and thereby downregulated by DNA damage [22]. In addition, the small EV secretion pathway also removes harmful cytoplasmic DNA fragments from cells [24,45]. However, the relationship between small EV release and autophagy in the regulation of cytoplasmic DNA fragments has remained unclear. Previous reports indicated that activating ceramide pathway blocks the autophagy-mediated degradation pathway [46]. Therefore, we speculated that DNA damage might block the autophagy pathway through ceramide pathway activation and, in turn, promote small EV release to prevent the accumulation of chromosomal DNA fragments in the cytoplasm of normal cells. We treated TIG-3 cells with autophagy pathway inhibitors that target lysosomes, chloroquine (CQ) and bafilomycin A1 (BafA1) [47]. Autophagy pathway inhibition caused an accumulation of chromosomal DNA fragments in the cytoplasm and cell cycle arrest in normal HDFs (Figure 4A–C). Significantly, the gene expression of a number of SASP factors was upregulated by these inhibitors (Figure 4D). Intriguingly, these treated cells also showed increases in the release of small EVs and double strand DNA (dsDNA) fragments from cells (Figure 4E,F). Similar to the situation in HDFs, DNA damage enhanced SASP-factor gene expression and small EV release in ATG5 knockout cells compared with their expression and release, respectively, in wild-type cells (WT) (Supplementary Figure S1) [48]. Research has previously shown that autophagy dysregulations can be detected in aged cells, and autophagy activation tended to improve senescent phenotypes [49,50]. Therefore, we treated senescent HDFs with rapamycin, an mTOR signaling inhibitor and autophagy inducer [51,52,53]. Strikingly, rapamycin treatment blocked IFN-β and CXCL10 expression in senescent cells (Supplementary Figure S2). Taken together, these data strongly indicated that downregulation of the autophagy pathway promotes small EV release for the secretion of harmful chromosomal DNA fragments from cells (Figure 4G).

2.5. Small EV Release and Autophagy Cooperatively Prevent Cell Death Caused by Bacterial Infection

Previously, we reported that small EV secretion prevented adenovirus infection by excluding viral DNA from cells [24]. Additionally, we assessed the interplay between the release of small EVs and autophagy in preventing inflammation caused by bacterial infection. After differentiation into mature macrophage-like cells by Phorbol 12-myristate 13-acae-tate (PMA) stimulation for 7 days, human monocytic leukemia cells (THP-1 cells) were then infected with Bacillus Calmette–Guérin (BCG) vaccine, which is an attenuated form of Mycobacterium bovis, with or without inhibiting small EV biogenesis or secretion using siRNA oligos against Alix or Rab27a, as previously described (Figure 5A,B) [24]. Bacterial infection activates inflammatory responses in host cells. Indeed, inhibiting the small EV pathway dramatically increased the expressions of inflammatory genes, such as IFN-β and CXCL10 (Figure 5C), resulting in apoptotic cell death (Figure 5D). Notably, the cleaved forms of both Caspase 3 and Caspase 1, markers of inflammasome activation, were clearly detected by the inhibition of small EV secretion in THP-1 cells following infection with BCG (Figure S3). Since bacterial DNA activates inflammasomes via the cGAS-STING pathway [54,55,56,57], STING depletion using previously validated siRNA oligos blocked both inflammatory gene expression and apoptotic cell death, suggesting that small EV release prevents excessive inflammatory responses caused by STING activation. The autophagy pathway also acts as a barrier against bacterial infection [58]. The levels of bacterial genomic DNA in host cells and small EV release increased considerably when autophagy was inhibited by adding 3-MA, an autophagy inhibitor (Figure S4A,B) [59]. Importantly, apoptotic cell death increased significantly by inhibiting both autophagy and EV biogenesis (Supplementary Figure S4C). Collectively, these results demonstrate that small EV release and autophagy function cooperatively to prevent cellular inflammatory responses against bacterial infection.

3. Discussion

Senescent cells are metabolically active in a state of stable cell cycle arrest; they accumulate in the living body during the aging process [9,10,11]. These cells have been reported to play both beneficial and deleterious roles in our health through secreting SASP factors [12,13,14,15,16,17], and they also release many types of EVs, such as exosomes, microvesicles, nucleosomes, and apoptotic bodies, which are characterized by their size and secretory machinery [60,61,62,63]. Previously, we and other groups have reported that small EVs are actively released from senescent cells, functioning as harmful SASP factors by regulating the growth and viability of cancer cells [24,25,31]. According to recent studies, the biological functions of small EVs released from senescent cells change drastically because of changes in the composition of their proteins, lipids, and nucleic acids during cellular senescence [25,26,60,62,63,64]. In this study, we demonstrated that DNA damage is a key trigger, not only of senescence induction but also of small EV biogenesis via ceramide synthesis in senescent cells. The most common downstream mediator of DNA damage signaling, p53, reportedly induces the expression of several genes involved in endosome regulation and promote small EVs production [65]. In agreement with a previous report, we observed that DNA damage increased nSMase2 expression in HDFs and epithelial cells, suggesting that p53 activation might be involved in this phenomenon [66]. Additionally, we discovered that the expression of SMS2, an antagonistic enzyme of nSMase2 ceramide synthesis, reduced dramatically during cellular senescence (Figure 1C,D,F,G). The activation of sphingolipid-metabolizing enzymes is important for clearing amyloid beta (Aβ) protein from the brain is associated with preventing Alzheimer’s disease [40]. Therefore, it would appear to be important to reveal the mechanism involved in regulating SMS2 expression by DNA damage, and further investigations are required.
Cytoplasmic DNA fragments, derived from endogenous chromosomal or mitochondrial DNA resulting from DNA damage or from exogenous viral or bacterial infection, are detected by specific DNA-sensing machinery, such as the cGAS-STING pathway. Recent studies have shown that the cytoplasmic DNA-sensing pathway is critical for SASP-factor gene expression in senescent cells [19,20,21,22,23]. The innate immune response is important in fighting viral or bacterial infections, although excessive activation of this pathway can be dangerous for cells because the sustained activation of inflammasomes can result in additional DNA damage and/or cell death. Therefore, both DNA degradation enzymes and autophagy work to clear harmful cytoplasmic DNA fragments. However, in senescent cells, these cellular fail-safe mechanisms may not function normally because of persistent DNA damage signaling. Thus, the EV-mediated secretion pathway may also play a role in clearing cytoplasmic DNA fragments (see the model in Figure 6).
Altogether, we have elucidated that DNA damage can provoke senescence-associated EV (SA-EV) secretion by activating the ceramide pathway, thereby helping to eliminate hazardous DNA fragments from cells. It is notable that there might be alternative mechanisms for SA-EV secretion, and these could be potential therapeutic targets for the prevention of SASP, along with senolytic drugs to eliminate senescent cells [67]. Therefore, we will conduct further studies to address the molecular mechanisms underlying SA-EV biogenesis.

4. Materials and Methods

4.1. Cell Culture

TIG-3 and RPE-1 cells were obtained from Japanese Cancer Research Resources Bank (JCRB, Osaka, Japan) and mouse primary fibroblasts (MEFs) were established from day 13.5 mouse embryos. Wild type (WT) and atg5-/- immortalized MEFs [48] were obtained from RIKEN Cell Bank (RCB2710 and RCB2711, respectively) (RIKEN BRC, Ibaraki, Japan). These cells were cultured in Dulbecco’s Modified Eagle’s (DME) medium (Nacalai Tesque, Kyoto, Japan) supplemented with 10% fetal bovine serum (FBS). THP-1 cells were obtained from Cell Resource Center for Biomedical Research, Tohoku University. They were cultured in RPMI 1620 medium (Nacalai Tesque) supplemented with 10% FBS. In this research, young control cells were less than 40 population doublings and replicative senescent cells were more than 70 population doublings. TIG-3 cells were infected with recombinant retroviruses encoding RasV12 (in pBabe–puro) or SMS2 or nSMase2 (in pMarX–puro) cDNA and treated with puromycin for 7 days [22]. For senescence induction, cells were irradiated with 10 Gy or 20 Gy X-rays using CP-160 (Faxitron X-ray Inc., Arizona, USA). An nSMase inhibitor GW4869 (Sigma-Aldrich, St. Louis, MO, USA), spiroepoxide (Santa Cruz, Dallas, TX, USA), doxorubicin (Wako, Osaka, Japan), chloroquine (Sigma-Aldrich), bafilomycin A1 (Sigma-Aldrich), rapamycin (Calbiochem, Merck, Darmstadt, Germany), PMA (Promega, Madison, WI, USA) or 3-MA (Calbiochem) were used in some experiments. Bacillus Calmette-Guérin (BCG) was purchased from Japan BCG Laboratory (Japan BCG Laboratory, Tokyo, Japan). All culture cells were confirmed the absence of mycoplasma contamination.

4.2. Cell Proliferation Assay

Cells were plated on 35 mm dishes with 2 mm grids (Thermo Fisher Scientific, Waltham, MA, USA). The number of cells in each grid was counted every day, and the relative number of cells was calculated based on an adjusted cell number at day 1 set at 1.0 as described previously [7].

4.3. Apoptosis Assay

Apoptotic cells were judged by FITC-Annexin V staining using an apoptotic/healthy cells detection kit (PromoKine, Heidelberg, Germany) as described previously [24]. After an incubation at room temperature for 15 min, fluorescence signals were measured with a Wallac ARVO 1420 Multilabel counter (PerkinElmer Co., Ltd., Waltham, MA, USA).

4.4. Cytoplasmic Nuclear DNA Analysis

Cytoplasmic DNA was prepared by modifying a method as previously reported [22,68]. In brief, cells were centrifuged for 1 min in a microcentrifuge, then suspended in 0.3 M sucrose buffer and homogenized with pipetting. The homogenate was overlaid on the same amount of 1.5 M sucrose buffer and centrifuged at 13,200 rpm for 10 min. Cytoplasmic DNA was purified by 0.4 mg/mL Proteinase K (Wako) treatment, phenol/chloroform extraction and ethanol precipitation with a carrier (Dr. GenTLE®, Takara Bio, Shiga, Japan). Cytoplasmic nuclear DNA was estimated by quantitative Real-Time PCR, using three different sets of primers as follows: human GRM7, 5′-TCAAGTGCCACATCCTATGC-3′ (forward), and 5′-ATTTTTCTAGCCAGGCACCA-3′ (reverse); human FGFR2, 5′-ACCTGGAAATGGCTGAAATG-3′ (forward), and 5′-AAGTCCTCGCAGAGGTTTCA-3′ (reverse); human GPC6, 5′-CGCCAGTGTGTGTAGCACTT-3′ (forward), and 5′-TCGGCCTCTCTCAGTTCTGT-3′ (reverse) [22].

4.5. Small Extracellular Vesicle Isolation from Cells

Small EVs were obtained from cell supernatants, as previously described with some modifications [24,27,69]. In brief, cells were incubated in DME medium with ultracentrifuged 5% FBS for 48 hours. The supernatants were collected and centrifuged at 300 g for 5 min and then at 2000× g for 10 min. The supernatant was then centrifuged at 10,000× g for 30 min, followed by filtration through a 0.2-μm pore filter (17597K, Sartorius, Gottingen, Lower Saxony, Germany). The collected supernatant was then subjected to preparation procedures by either ultracentrifugation at 100,000× g for 70 min as previously described [24,25] or an affinity-based method using MagCapture (Fujifilm Wako Chemicals, Tokyo, Japan) [70] for small EVs isolation. Nanoparticle tracking analysis were performed using a NanoSight LM10 system (Malvern Panalytical, Westborough, MA, USA). The amount of dsDNA in EVs was determined by quantitative Real-Time PCR using these primers: human LINE1, 5′-CAAACACCGCATATTCTCACTCA-3′ (forward), and 5′-CTTCCTGTGTCCATGTGATCTCA-3′ (reverse) [23,24].

4.6. Fluorescence Microscopic Analysis

The cells were fixed with 4% paraformaldehyde/PBS (Wako) and permeated through the membrane with 0.5% Triton X-100/tris-buffered saline (TBS) for 1 minutes. The cells were blocked with 1% bovine serum albumin (BSA) and 10% goat serum/TBS for 1 hour at 4 °C. Then, it was made to react with the following antibodies: γH2AX (1: 1,000, 05-636, Millipore, Temecula, CA, USA), phospho-(Ser/Thr) ATM/ATR substrate (1: 500, 2851, Cell Signaling Technology, Danver MA, USA), 53BP1 (1: 250, sc-58749, Santa Cruz). The secondary antibody was reacted using Alexa488 and Alexa594 (Thermo Fisher Scientific), and the nucleus was stained using DAPI (Dojindo, Tokyo, Japan). After immunostaining, DNA damage-positive cells were quantified by observation using a fluorescence microscope (Carl Zeiss, Oberkochen, Germany).

4.7. Electron Microscopy

Small EVs isolated from RPE-1 cells were absorbed to formvar carbon coated nickel grids and immune-labelled with an anti-CD63 antibody (556019, BD Biosciences, NJ, USA), followed by 5 nM of a gold-labelled secondary antibody (British BioCell International Ltd., UK). The samples were fixed in 2% glutaraldehyde in 0.1 M phosphate buffer. The grids were placed in 2% glutaraldehyde in 0.1 M phosphate buffer and dried, then stained with 2% uranyl acetate for 15 min and a Lead stain solution (Sigma-Aldrich). The samples were observed with a transmission electron microscope (JEM-1400Plus, JEOL Ltd., Tokyo, Japan) at 80 kV. Digital images were obtained with a CCD camera (VELETA, Olympus Soft imaging solutions GmbH, Olympus, Tokyo, Japan) [24].

4.8. RNAi

The sequences of the siRNA oligos were as follows. SMS2 [43]: GGGCAUUGCCUUCAUAUAU. nSMase2 [38]: GGAGGUGUUUGACAAGCG. Alix [24,36,38]: GAACCUGGAUAAUGAUGAA. Rab27a [24,35]: GCUGCCAAUGGGACAAACA. ON-TARGETplus siRNAs to target Sting mRNA sequences and non-targeting control siRNA were used (Dharmacon, Waterbeach, Cambridge, UK) [22,71].

4.9. Plasmids

The epitope tagged cDNAs of SMS2 and nSMase2 was cloned into the pMarX-puro retrovirus vector. All cDNAs were sequenced on a Genetic Analyzer 3130 (Applied Biosystems, Waltham, MA, USA) using a BigDye Terminator v3.1 Cycle Sequencing Kit (Applied Biosystems).

4.10. Quantitative Real-Time PCR

Total RNA was prepared using a mirVana kit (Thermo Fisher Scientific), and then subjected to reverse transcription using a PrimeScript RT reagent kit (Takara Bio Inc., Shiga, Japan). The expression levels of each mRNA were examined by quantitative real-time RT-PCR on a StepOnePlus PCR system (Applied Biosystems) using SYBR Premix Ex Taq (Takara Bio Inc.). The PCR primer sequences used are as follows: human GAPDH, 5′-CAACTACATGGTTTACATGTTC-3′ (forward) and 5′-GCCAGTGGACTCCACGAC-3′ (reverse) [22]; human p16 (cdkn2a), 5′-CGAATAGTTACGGTCGGAGG-3′ (forward) and 5′-TGAGAGTGGCGGGGTCG-3′ (reverse) [22]; human p21 (cdkn1a), 5′-TCAGGGTCGAAAACGGCG-3′ (forward) and 5′-AAGATCAGCCGGCGTTTGGA-3′ (reverse) [18]; SMS2, 5′-AGGAGCTTAGCCCTCCACTC-3′ (forward) and 5′-AACAGAATCTGCGTCCCACT-3′ (reverse); nSMase2, 5′-CAACAAGTGTAACGACGATGCC-3′ (forward) and 5′-GGCATCGTCGTTACACTTGTTG-3′ (reverse) [72]; human IL-6, 5′-CCAGGAGCCCAGCTATGAAC-3′ (forward) and 5′-CCCAGGGAGAAGGCAACTG-3′ (reverse) [22]; IL-8, 5′-AAGGAAAACTGGGTGCAGAG-3′ (forward) and 5′-ATTGCATCTGGCAACCCTAC-3′ (reverse) [22]; human IL-1α, 5′-AACCAGTGCTGCTGAAGGA-3′(forward) and 5′-TTCTTAGTGCCGTGAGTTTCC-3′ (reverse) [22]; human IL-1β, 5′-CTGTCCTGCGTGTTGAAAGA-3′ (forward) and 5′-TTGGGTAATTTTTGGGATCTACA-3′ (reverse) [22]; human IFN-β, 5′-AAACTCATGAGCAGTCTGCA-3′ (forward) and 5′-AGGAGATCTTCAGTTTCGGAGG-3′ (reverse) [22]; human CXCL10, 5′-CCAGAATCGAAGGCCATCAA-3′ (forward) and 5′-CATTTCCTTGCTAACTGCTTTCAG-3′ (reverse) [22]; human Alix, 5′-CCCAAATTCCCATTTTCTGA-3′ (forward) and 5′-GAGCCTCCAAAAAGTGAACC-3′ (reverse) [24]; human Rab27a, 5′-ATCACAACAGTGGGCATTGA-3′ (forward) and 5′-CCCTGCTGTGTCCCATAACT-3′ (reverse) [24]; human STING, 5′-ATATCTGCGGCTGATCCTGC-3′ (forward) and 5′-GGTCTGCTGGGGCAGTTTAT-3′ (reverse) [19]; mouse GAPDH, 5′-CAACTACATGGTCTACATGTTC-3′ (forward) and 5′-CGCCAGTAGACTCCACGAC-3′ (reverse) [22]; mouse p16, 5′-GAACTCTTTCGGTCGTACCC-3′ (forward) and 5′-CGAATCTGCACCGTAGTTGA-3′ (reverse) [22]; mouse IL-6, 5′-CCGGAGAGGAGACTTCACAG-3′ (forward) and 5′-TCCACGATTTCCCAGAGAAC-3′ (reverse) [22]; mouse GRO-α, 5′-CCGCTCGCTTCTCTGTGC-3′ (forward) and 5′-CTCTGGATGTTCTTGAGGTGAATC-3′ (reverse) [18]; mouse IFN-β, 5′-CAGCTCCAAGAAAGGACGAAC-3′ (forward) and 5′-GGCAGTGTAACTCTTCTGCAT-3′ (reverse) [22]; mouse CXCL10, 5′-CCAAGTGCTGCCGTCATTTTC-3′ (forward) and 5′-GGCTCGCAGGGATGATTTCAA-3′ (reverse) [22]; BCG, 5′-GTCCACGCCGCCAACTACG-3′ (forward) and 5′-GTTAGGTGCTGGTGGTCCGAAG-3′ (reverse) [73]. The means ± s.d. of three independent experiments are shown.

4.11. Western Blotting

For Western blotting analysis, cells were lysed in lysis buffer (50 mM Hepes, pH 7.5, 150 mM NaCl, 1 mM EDTA, 2.5 mM EGTA, 10% glycerol, 0.1% Tween20, 10 mM β-glycerophosphate) with 1% Protease inhibitor cocktail (Nacalai Tesque). The protein concentration was determined using a Pierce™ BCA Protein Assay Kit (23225, Thermo Fisher Scientific), and the proteins were transferred to a PVDF membrane (EMD Millipore) after SDS-PAGE. Primary antibodies used in this study were anti-SMS2 (sc-366682, Santa Cruz), nSMase2 (sc-166637, Santa Cruz), H-Ras (sc-29, Santa Cruz), Alix (12422, Proteintech, Rosemont, IL, USA), Rab27a (17817, Proteintech), Caspase3 (9662, Cell Signaling Technology), Caspase1 (sc-1780, Santa Cruz), ATG5 (12994, Cell Signaling Technology), p62 (PM045, MBL International, Woburn, MA, USA), LC3 (2775, Cell Signal Transduction), α-tubulin (T9026, Sigma-Aldrich). After incubation with secondary antibodies (GE Healthcare, Chicago, IL, USA), membranes were treated with the SuperSignal West Femto Maximum Sensitivity Substrate (Thermo Fisher Scientific), and detected by FUSION SOLO S (Vilber Lourmat, Collegien, France).

4.12. Animal Experiments

CD1 (ICR) mice were purchased from Charles River Inc. (Wilmington, MA, USA). An N-SMase inhibitor, spiroepoxide (Santa Cruz), was intraperitoneally injected into 50-day-old male mice at 3.5 mg/kg every two day. Fourteen days later, mice treated with spiroepoxide were euthanized and the small intestine sections were subjected to small EV collection or immunofluorescence analysis as described previously [24]. All animal care was performed according to the protocols approved by the Committee for the Use and Care of Experimental Animals of the Japanese Foundation for Cancer Research (No.17-02-1, 31 5 2017).

4.13. Statistical Analysis

Statistical significance was determined using unpaired two-tailed Student’s t-test by Excell (Microsoft, Redmond, WA, USA). p-values less than 0.05 were considered significant.

5. Conclusions

We demonstrated how DNA damage activates the ceramide pathway and leads to increase senescence-associated EV (SA-EV) secretion. The SA-EV pathway is crucial for cellular homeostasis to protect cells from excessive inflammatory responses.

Supplementary Materials

The following are available online at https://www.mdpi.com/1422-0067/21/10/3720/s1, Figure S1: DNA damage enhanced small EV release from ATG5 knockout mouse embryonic fibroblasts (MEFs) compared with their release in wild-type MEFs. Figure S2: Activation of the autophagy pathway prevents inflammatory gene expression in senescent cells. Figure S3: Inhibiting the small EV pathway provokes inflammasome activation and apoptosis in Bacillus Calmette-Guérin (BCG)-infected cells. Figure S4: Inhibiting both autophagy and small EV biogenesis promotes apoptotic cell death following Bacillus Calmette-Guérin (BCG) infection.

Author Contributions

K.H., R.O. and A.T. designed the experiments. K.H., R.O., T.M.L., K.M. and A.T. performed the experiments. K.H., R.O., T.M.L., K.M., A.J.N. and A.T. analysed the data. K.H. and A.T. wrote the manuscript. A.T. oversaw the projects. All authors have read and agreed to the published version of the manuscript.

Funding

This research was supported in part by grants from Japan Science and Technology Agency (JST)-PRESTO under grant number JPMJPR17H7, from Japan Agency of Medical Research and Development (AMED) under grant number 19gm6110023h0001 and from Japan Society for the Promotion of Science (JSPS) under grant number 17K19618, 18K15073, 19H03507, 20K16163, 20K16344, the Vehicle Racing Commemorative Foundation, Takeda Science Foundation and the Mitsubishi Foundation.

Acknowledgments

We thank Eiji Hara (Professor, Osaka University) for helpful discussion during the preparation of this manuscript; Noboru Mizushima (Professor, The University of Tokyo) for providing the WT and atg5-/-MEF cells; Yosuke Ishihara (Tokai-Denshi Inc., Sizuoka, Japan) for technical supports for TEM analysis.

Conflicts of Interest

The authors declare no competing financial interests.

Abbreviations

DDRDNA damage response
EVExtracellular vesicle
NTANanoparticle tracking analysis
SASPSenescence-associated secretory phenotype
cGASThe cyclic GMP-AMP synthase
STINGStimulator of interferon genes
WTWild-type
dsDNADouble strand DNA

References

  1. Campisi, J.; d’Adda di Fagagna, F. Cellular senescence: When bad things happen to good cells. Nat. Rev. Mol. Cell Biol. 2007, 8, 729–740. [Google Scholar] [CrossRef] [PubMed]
  2. White, R.R.; Vijg, J. Do DNA Double-Strand Breaks Drive Aging? Mol. Cell 2016, 63, 729–738. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  3. Takeuchi, S.; Takahashi, A.; Motoi, N.; Yoshimoto, S.; Tajima, T.; Yamakoshi, K.; Hirao, A.; Yanagi, S.; Fukami, K.; Ishikawa, Y.; et al. Intrinsic cooperation between p16INK4a and p21Waf1/Cip1 in the onset of cellular senescence and tumor suppression in vivo. Cancer Res. 2010, 70, 9381–9390. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  4. He, S.; Sharpless, N.E. Senescence in Health and Disease. Cell 2017, 169, 1000–1011. [Google Scholar] [CrossRef]
  5. Gorgoulis, V.; Adams, P.D.; Alimonti, A.; Bennett, D.C.; Bischof, O.; Bishop, C.; Campisi, J.; Collado, M.; Evangelou, K.; Ferbeyre, G.; et al. Cellular Senescence: Defining a Path Forward. Cell 2019, 179, 813–827. [Google Scholar] [CrossRef]
  6. Maehara, K.; Yamakoshi, K.; Ohtani, N.; Kubo, Y.; Takahashi, A.; Arase, S.; Jones, N.; Hara, E. Reduction of total E2F/DP activity induces senescence-like cell cycle arrest in cancer cells lacking functional pRB and p53. J. Cell Biol. 2005, 168, 553–560. [Google Scholar] [CrossRef] [Green Version]
  7. Takahashi, A.; Ohtani, N.; Yamakoshi, K.; Iida, S.; Tahara, H.; Nakayama, K.; Nakayama, K.I.; Ide, T.; Saya, H.; Hara, E. Mitogenic signalling and the p16INK4a-Rb pathway cooperate to enforce irreversible cellular senescence. Nat. Cell Biol. 2006, 8, 1291–1297. [Google Scholar] [CrossRef]
  8. Imai, Y.; Takahashi, A.; Hanyu, A.; Hori, S.; Sato, S.; Naka, K.; Hirao, A.; Ohtani, N.; Hara, E. Crosstalk between the Rb pathway and AKT signaling forms a quiescence-senescence switch. Cell Rep. 2014, 7, 194–207. [Google Scholar] [CrossRef] [Green Version]
  9. Ohtani, N.; Imamura, Y.; Yamakoshi, K.; Hirota, F.; Nakayama, R.; Kubo, Y.; Ishimaru, N.; Takahashi, A.; Hirao, A.; Shimizu, T.; et al. Visualizing the dynamics of p21(Waf1/Cip1) cyclin-dependent kinase inhibitor expression in living animals. Proc. Natl. Acad. Sci. USA 2007, 104, 15034–15039. [Google Scholar] [CrossRef] [Green Version]
  10. Yamakoshi, K.; Takahashi, A.; Hirota, F.; Nakayama, R.; Ishimaru, N.; Kubo, Y.; Mann, D.J.; Ohmura, M.; Hirao, A.; Saya, H.; et al. Real-time in vivo imaging of p16Ink4a reveals cross talk with p53. J. Cell Biol. 2009, 186, 393–407. [Google Scholar] [CrossRef] [Green Version]
  11. Burd, C.E.; Sorrentino, J.A.; Clark, K.S.; Darr, D.B.; Krishnamurthy, J.; Deal, A.M.; Bardeesy, N.; Castrillon, D.H.; Beach, D.H.; Sharpless, N.E. Monitoring tumorigenesis and senescence in vivo with a p16(INK4a)-luciferase model. Cell 2013, 152, 340–351. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  12. Kuilman, T.; Michaloglou, C.; Mooi, W.J.; Peeper, D.S. The essence of senescence. Genes Dev. 2010, 24, 2463–2479. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  13. Munoz-Espin, D.; Serrano, M. Cellular senescence: From physiology to pathology. Nat. Rev. Mol. Cell Biol. 2014, 15, 482–496. [Google Scholar] [CrossRef]
  14. Childs, B.G.; Gluscevic, M.; Baker, D.J.; Laberge, R.M.; Marquess, D.; Dananberg, J.; van Deursen, J.M. Senescent cells: An emerging target for diseases of ageing. Nat. Rev. Drug Discov. 2017, 16, 718–735. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  15. Faget, D.V.; Ren, Q.; Stewart, S.A. Unmasking senescence: Context-dependent effects of SASP in cancer. Nat. Rev. Cancer 2019, 19, 439–453. [Google Scholar] [CrossRef]
  16. Loo, T.M.; Miyata, K.; Tanaka, Y.; Takahashi, A. Cellular senescence and senescence-associated secretory phenotype via the cGAS-STING signaling pathway in cancer. Cancer Sci. 2020, 111, 304–311. [Google Scholar] [CrossRef] [Green Version]
  17. Rodier, F.; Campisi, J. Four faces of cellular senescence. J. Cell Biol. 2011, 192, 547–556. [Google Scholar] [CrossRef]
  18. Takahashi, A.; Imai, Y.; Yamakoshi, K.; Kuninaka, S.; Ohtani, N.; Yoshimoto, S.; Hori, S.; Tachibana, M.; Anderton, E.; Takeuchi, T.; et al. DNA damage signaling triggers degradation of histone methyltransferases through APC/C(Cdh1) in senescent cells. Mol. Cell 2012, 45, 123–131. [Google Scholar] [CrossRef] [Green Version]
  19. Dou, Z.; Ghosh, K.; Vizioli, M.G.; Zhu, J.; Sen, P.; Wangensteen, K.J.; Simithy, J.; Lan, Y.; Lin, Y.; Zhou, Z.; et al. Cytoplasmic chromatin triggers inflammation in senescence and cancer. Nature 2017, 550, 402–406. [Google Scholar] [CrossRef] [Green Version]
  20. Gluck, S.; Guey, B.; Gulen, M.F.; Wolter, K.; Kang, T.W.; Schmacke, N.A.; Bridgeman, A.; Rehwinkel, J.; Zender, L.; Ablasser, A. Innate immune sensing of cytosolic chromatin fragments through cGAS promotes senescence. Nat. Cell Biol. 2017, 19, 1061–1070. [Google Scholar] [CrossRef]
  21. Yang, H.; Wang, H.; Ren, J.; Chen, Q.; Chen, Z.J. cGAS is essential for cellular senescence. Proc. Natl. Acad. Sci. USA 2017, 114, 4612–4620. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  22. Takahashi, A.; Loo, T.M.; Okada, R.; Kamachi, F.; Watanabe, Y.; Wakita, M.; Watanabe, S.; Kawamoto, S.; Miyata, K.; Barber, G.N.; et al. Downregulation of cytoplasmic DNases is implicated in cytoplasmic DNA accumulation and SASP in senescent cells. Nat. Commun. 2018, 9, 1249. [Google Scholar] [CrossRef] [PubMed]
  23. De Cecco, M.; Ito, T.; Petrashen, A.P.; Elias, A.E.; Skvir, N.J.; Criscione, S.W.; Caligiana, A.; Brocculi, G.; Adney, E.M.; Boeke, J.D.; et al. L1 drives IFN in senescent cells and promotes age-associated inflammation. Nature 2019, 566, 73–78. [Google Scholar] [CrossRef] [PubMed]
  24. Takahashi, A.; Okada, R.; Nagao, K.; Kawamata, Y.; Hanyu, A.; Yoshimoto, S.; Takasugi, M.; Watanabe, S.; Kanemaki, M.T.; Obuse, C.; et al. Exosomes maintain cellular homeostasis by excreting harmful DNA from cells. Nat. Commun. 2017, 8, 15287. [Google Scholar] [CrossRef] [Green Version]
  25. Takasugi, M.; Okada, R.; Takahashi, A.; Virya Chen, D.; Watanabe, S.; Hara, E. Small extracellular vesicles secreted from senescent cells promote cancer cell proliferation through EphA2. Nat. Commun. 2017, 8, 15729. [Google Scholar] [CrossRef]
  26. Riquelme, J.A.; Takov, K.; Santiago-Fernandez, C.; Rossello, X.; Lavandero, S.; Yellon, D.M.; Davidson, S.M. Increased production of functional small extracellular vesicles in senescent endothelial cells. J. Cell. Mol. Med. 2020, 24, 4871–4876. [Google Scholar] [CrossRef] [Green Version]
  27. Valadi, H.; Ekstrom, K.; Bossios, A.; Sjostrand, M.; Lee, J.J.; Lotvall, J.O. Exosome-mediated transfer of mRNAs and microRNAs is a novel mechanism of genetic exchange between cells. Nat. Cell Biol. 2007, 9, 654–659. [Google Scholar] [CrossRef] [Green Version]
  28. Raposo, G.; Stoorvogel, W. Extracellular vesicles: Exosomes, microvesicles, and friends. J. Cell Biol. 2013, 200, 373–383. [Google Scholar] [CrossRef] [Green Version]
  29. Tkach, M.; Thery, C. Communication by Extracellular Vesicles: Where We Are and Where We Need to Go. Cell 2016, 164, 1226–1232. [Google Scholar] [CrossRef] [Green Version]
  30. Jakhar, R.; Crasta, K. Exosomes as Emerging Pro-Tumorigenic Mediators of the Senescence-Associated Secretory Phenotype. Int. J. Mol. Sci. 2019, 20, 2547. [Google Scholar] [CrossRef] [Green Version]
  31. Miyazoe, Y.; Miuma, S.; Miyaaki, H.; Kanda, Y.; Nakashiki, S.; Sasaki, R.; Haraguchi, M.; Shibata, H.; Honda, T.; Taura, N.; et al. Extracellular vesicles from senescent hepatic stellate cells promote cell viability of hepatoma cells through increasing EGF secretion from differentiated THP-1 cells. Biomed. Rep. 2020, 12, 163–170. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  32. Lehmann, B.D.; Paine, M.S.; Brooks, A.M.; McCubrey, J.A.; Renegar, R.H.; Wang, R.; Terrian, D.M. Senescence-associated exosome release from human prostate cancer cells. Cancer Res. 2008, 68, 7864–7871. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  33. Moertl, S.; Buschmann, D.; Azimzadeh, O.; Schneider, M.; Kell, R.; Winkler, K.; Tapio, S.; Hornhardt, S.; Merl-Pham, J.; Pfaffl, M.W.; et al. Radiation Exposure of Peripheral Mononuclear Blood Cells Alters the Composition and Function of Secreted Extracellular Vesicles. Int. J. Mol. Sci. 2020, 21, 2336. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  34. Trajkovic, K.; Hsu, C.; Chiantia, S.; Rajendran, L.; Wenzel, D.; Wieland, F.; Schwille, P.; Brugger, B.; Simons, M. Ceramide triggers budding of exosome vesicles into multivesicular endosomes. Science 2008, 319, 1244–1247. [Google Scholar] [CrossRef] [PubMed]
  35. Ostrowski, M.; Carmo, N.B.; Krumeich, S.; Fanget, I.; Raposo, G.; Savina, A.; Moita, C.F.; Schauer, K.; Hume, A.N.; Freitas, R.P.; et al. Rab27a and Rab27b control different steps of the exosome secretion pathway. Nat. Cell Biol. 2010, 12, 19–30. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  36. Baietti, M.F.; Zhang, Z.; Mortier, E.; Melchior, A.; Degeest, G.; Geeraerts, A.; Ivarsson, Y.; Depoortere, F.; Coomans, C.; Vermeiren, E.; et al. Syndecan–syntenin–ALIX regulates the biogenesis of exosomes. Nat. Cell Biol. 2012, 14, 677–685. [Google Scholar] [CrossRef]
  37. Colombo, M.; Moita, C.; van Niel, G.; Kowal, J.; Vigneron, J.; Benaroch, P.; Manel, N.; Moita, L.F.; Thery, C.; Raposo, G. Analysis of ESCRT functions in exosome biogenesis, composition and secretion highlights the heterogeneity of extracellular vesicles. J. Cell Sci. 2013, 126, 5553–5565. [Google Scholar] [CrossRef] [Green Version]
  38. Kosaka, N.; Iguchi, H.; Yoshioka, Y.; Takeshita, F.; Matsuki, Y.; Ochiya, T. Secretory mechanisms and intercellular transfer of microRNAs in living cells. J. Biol. Chem. 2010, 285, 17442–17452. [Google Scholar] [CrossRef] [Green Version]
  39. Mittelbrunn, M.; Sánchez-Madrid, F. Intercellular communication: Diverse structures for exchange of genetic information. Nat. Rev. Mol. Cell Biol. 2012, 13, 328–335. [Google Scholar] [CrossRef]
  40. Yuyama, K.; Sun, H.; Mitsutake, S.; Igarashi, Y. Sphingolipid-modulated exosome secretion promotes clearance of amyloid-beta by microglia. J. Biol. Chem. 2012, 287, 10977–10989. [Google Scholar] [CrossRef] [Green Version]
  41. Li, J.; Liu, K.; Liu, Y.; Xu, Y.; Zhang, F.; Yang, H.; Liu, J.; Pan, T.; Chen, J.; Wu, M.; et al. Exosomes mediate the cell-to-cell transmission of IFN-alpha-induced antiviral activity. Nat. Immunol. 2013, 14, 793–803. [Google Scholar] [CrossRef] [PubMed]
  42. Pols, M.S.; Klumperman, J. Trafficking and function of the tetraspanin CD63. Exp. Cell Res. 2009, 315, 1584–1592. [Google Scholar] [CrossRef] [PubMed]
  43. Mitsutake, S.; Zama, K.; Yokota, H.; Yoshida, T.; Tanaka, M.; Mitsui, M.; Ikawa, M.; Okabe, M.; Tanaka, Y.; Yamashita, T.; et al. Dynamic modification of sphingomyelin in lipid microdomains controls development of obesity, fatty liver, and type 2 diabetes. J. Biol. Chem. 2011, 286, 28544–28555. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  44. Lan, Y.Y.; Londono, D.; Bouley, R.; Rooney, M.S.; Hacohen, N. Dnase2a deficiency uncovers lysosomal clearance of damaged nuclear DNA via autophagy. Cell Rep. 2014, 9, 180–192. [Google Scholar] [CrossRef] [Green Version]
  45. Asada, K.; Ito, K.; Yui, D.; Tagaya, H.; Yokota, T. Cytosolic Genomic DNA functions as a Natural Antisense. Sci. Rep. 2018, 8, 8551. [Google Scholar] [CrossRef]
  46. Orsini, M.; Chateauvieux, S.; Rhim, J.; Gaigneaux, A.; Cheillan, D.; Christov, C.; Dicato, M.; Morceau, F.; Diederich, M. Sphingolipid-mediated inflammatory signaling leading to autophagy inhibition converts erythropoiesis to myelopoiesis in human hematopoietic stem/progenitor cells. Cell Death Differ. 2019, 26, 1796–1812. [Google Scholar] [CrossRef] [Green Version]
  47. Redmann, M.; Benavides, G.A.; Berryhill, T.F.; Wani, W.Y.; Ouyang, X.; Johnson, M.S.; Ravi, S.; Barnes, S.; Darley-Usmar, V.M.; Zhang, J. Inhibition of autophagy with bafilomycin and chloroquine decreases mitochondrial quality and bioenergetic function in primary neurons. Redox Biol. 2017, 11, 73–81. [Google Scholar] [CrossRef] [Green Version]
  48. Kuma, A.; Hatano, M.; Matsui, M.; Yamamoto, A.; Nakaya, H.; Yoshimori, T.; Ohsumi, Y.; Tokuhisa, T.; Mizushima, N. The role of autophagy during the early neonatal starvation period. Nature 2004, 432, 1032–1036. [Google Scholar] [CrossRef]
  49. Kang, C.; Xu, Q.; Martin, T.D.; Li, M.Z.; Demaria, M.; Aron, L.; Lu, T.; Yankner, B.A.; Campisi, J.; Elledge, S.J. The DNA damage response induces inflammation and senescence by inhibiting autophagy of GATA4. Science 2015, 349, aaa5612. [Google Scholar] [CrossRef] [Green Version]
  50. Leidal, A.M.; Levine, B.; Debnath, J. Autophagy and the cell biology of age-related disease. Nat. Cell Biol. 2018, 20, 1338–1348. [Google Scholar] [CrossRef]
  51. Jung, C.H.; Ro, S.H.; Cao, J.; Otto, N.M.; Kim, D.H. mTOR regulation of autophagy. FEBS Lett. 2010, 584, 1287–1295. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  52. Herranz, N.; Gallage, S.; Mellone, M.; Wuestefeld, T.; Klotz, S.; Hanley, C.J.; Raguz, S.; Acosta, J.C.; Innes, A.J.; Banito, A.; et al. mTOR regulates MAPKAPK2 translation to control the senescence-associated secretory phenotype. Nat. Cell Biol. 2015, 17, 1205–1217. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  53. Laberge, R.M.; Sun, Y.; Orjalo, A.V.; Patil, C.K.; Freund, A.; Zhou, L.; Curran, S.C.; Davalos, A.R.; Wilson-Edell, K.A.; Liu, S.; et al. MTOR regulates the pro-tumorigenic senescence-associated secretory phenotype by promoting IL1A translation. Nat. Cell Biol. 2015, 17, 1049–1061. [Google Scholar] [CrossRef] [PubMed]
  54. Collins, A.C.; Cai, H.; Li, T.; Franco, L.H.; Li, X.D.; Nair, V.R.; Scharn, C.R.; Stamm, C.E.; Levine, B.; Chen, Z.J.; et al. Cyclic GMP-AMP Synthase Is an Innate Immune DNA Sensor for Mycobacterium tuberculosis. Cell Host Microbe 2015, 17, 820–828. [Google Scholar] [CrossRef] [Green Version]
  55. Wassermann, R.; Gulen, M.F.; Sala, C.; Perin, S.G.; Lou, Y.; Rybniker, J.; Schmid-Burgk, J.L.; Schmidt, T.; Hornung, V.; Cole, S.T.; et al. Mycobacterium tuberculosis Differentially Activates cGAS- and Inflammasome-Dependent Intracellular Immune Responses through ESX-1. Cell Host Microbe 2015, 17, 799–810. [Google Scholar] [CrossRef] [Green Version]
  56. Watson, R.O.; Bell, S.L.; MacDuff, D.A.; Kimmey, J.M.; Diner, E.J.; Olivas, J.; Vance, R.E.; Stallings, C.L.; Virgin, H.W.; Cox, J.S. The Cytosolic Sensor cGAS Detects Mycobacterium tuberculosis DNA to Induce Type I Interferons and Activate Autophagy. Cell Host Microbe 2015, 17, 811–819. [Google Scholar] [CrossRef] [Green Version]
  57. Barber, G.N. STING-dependent cytosolic DNA sensing pathways. Trends Immunol. 2014, 35, 88–93. [Google Scholar] [CrossRef]
  58. Sergeeva, O.A.; van der Goot, F.G. Kicking Out Pathogens in Exosomes. Cell 2015, 161, 1241–1242. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  59. Wu, Y.T.; Tan, H.L.; Shui, G.; Bauvy, C.; Huang, Q.; Wenk, M.R.; Ong, C.N.; Codogno, P.; Shen, H.M. Dual role of 3-methyladenine in modulation of autophagy via different temporal patterns of inhibition on class I and III phosphoinositide 3-kinase. J. Biol. Chem. 2010, 285, 10850–10861. [Google Scholar] [CrossRef] [Green Version]
  60. Buratta, S.; Urbanelli, L.; Sagini, K.; Giovagnoli, S.; Caponi, S.; Fioretto, D.; Mitro, N.; Caruso, D.; Emiliani, C. Extracellular vesicles released by fibroblasts undergoing H-Ras induced senescence show changes in lipid profile. PLoS ONE 2017, 12, e0188840. [Google Scholar] [CrossRef]
  61. Jeppesen, D.K.; Fenix, A.M.; Franklin, J.L.; Higginbotham, J.N.; Zhang, Q.; Zimmerman, L.J.; Liebler, D.C.; Ping, J.; Liu, Q.; Evans, R.; et al. Reassessment of Exosome Composition. Cell 2019, 177, 428–445.e18. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  62. Alibhai, F.J.; Lim, F.; Yeganeh, A.; DiStefano, P.V.; Binesh-Marvasti, T.; Belfiore, A.; Wlodarek, L.; Gustafson, D.; Millar, S.; Li, S.H.; et al. Cellular senescence contributes to age-dependent changes in circulating extracellular vesicle cargo and function. Aging Cell 2020, 19, e13103. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  63. Basisty, N.; Kale, A.; Jeon, O.H.; Kuehnemann, C.; Payne, T.; Rao, C.; Holtz, A.; Shah, S.; Sharma, V.; Ferrucci, L.; et al. A proteomic atlas of senescence-associated secretomes for aging biomarker development. PLoS Biol. 2020, 18, e3000599. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  64. Yoshida, M.; Satoh, A.; Lin, J.B.; Mills, K.F.; Sasaki, Y.; Rensing, N.; Wong, M.; Apte, R.S.; Imai, S.I. Extracellular Vesicle-Contained eNAMPT Delays Aging and Extends Lifespan in Mice. Cell Metab. 2019, 30, 329–342.e5. [Google Scholar] [CrossRef]
  65. Yu, X.; Riley, T.; Levine, A.J. The regulation of the endosomal compartment by p53 the tumor suppressor gene. FEBS J. 2009, 276, 2201–2212. [Google Scholar] [CrossRef] [PubMed]
  66. Shamseddine, A.A.; Clarke, C.J.; Carroll, B.; Airola, M.V.; Mohammed, S.; Rella, A.; Obeid, L.M.; Hannun, Y.A. P53-dependent upregulation of neutral sphingomyelinase-2: Role in doxorubicin-induced growth arrest. Cell Death Dis. 2015, 6, e1947. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  67. Wakita, M.; Takahashi, A.; Sano, O.; Loo, T.M.; Imai, Y.; Narukawa, M.; Iwata, H.; Matsudaira, T.; Kawamoto, S.; Ohtani, N.; et al. A BET family protein degrader provokes senolysis by targeting NHEJ and autophagy in senescent cells. Nat. Commun. 2020, 11, 1935. [Google Scholar] [CrossRef] [Green Version]
  68. Kawashima, A.; Tanigawa, K.; Akama, T.; Wu, H.; Sue, M.; Yoshihara, A.; Ishido, Y.; Kobiyama, K.; Takeshita, F.; Ishii, K.J.; et al. Fragments of genomic DNA released by injured cells activate innate immunity and suppress endocrine function in the thyroid. Endocrinology 2011, 152, 1702–1712. [Google Scholar] [CrossRef] [Green Version]
  69. Thery, C.; Amigorena, S.; Raposo, G.; Clayton, A. Isolation and characterization of exosomes from cell culture supernatants and biological fluids. Curr. Protoc. Cell Biol. 2006, 30, 3.22.1–3.22.29. [Google Scholar] [CrossRef]
  70. Yoshida, T.; Ishidome, T.; Hanayama, R. High Purity Isolation and Sensitive Quantification of Extracellular Vesicles Using Affinity to TIM4. Curr. Protoc. Cell Biol. 2017, 77, 3.45.1–3.45.18. [Google Scholar] [CrossRef]
  71. Hartlova, A.; Erttmann, S.F.; Raffi, F.A.; Schmalz, A.M.; Resch, U.; Anugula, S.; Lienenklaus, S.; Nilsson, L.M.; Kroger, A.; Nilsson, J.A.; et al. DNA damage primes the type I interferon system via the cytosolic DNA sensor STING to promote anti-microbial innate immunity. Immunity 2015, 42, 332–343. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  72. Marchesini, N.; Osta, W.; Bielawski, J.; Luberto, C.; Obeid, L.M.; Hannun, Y.A. Role for mammalian neutral sphingomyelinase 2 in confluence-induced growth arrest of MCF7 cells. J. Biol. Chem. 2004, 279, 25101–25111. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  73. Papaparaskevas, J.; Houhoula, D.P.; Siatelis, A.; Tsakris, A. Molecular-beacon-based real-time PCR for detection and quantification of Mycobacterium tuberculosis DNA in clinical samples. J. Clin. Microbiol. 2008, 46, 3177–3178. [Google Scholar] [CrossRef] [PubMed] [Green Version]
Ijms 21 03720 g001 550
Figure 1. Gene expression associated with the ceramide synthetic pathway is changed by damage to DNA. (A,B) TIG-3 cells were treated with doxorubicin (DXR) for 48h and subjected to immunofluorescence staining for markers of DNA damage (γ-H2AX [red], phosphor-Ser/Thr ATM/ATR (pST/Q) substrate [green] and 40,6-diamidino-2-phenylindole: DAPI [blue]) (A) or to NanoSight analysis of isolated sEV particles (B). (C,D) Pre-senescent TIG-3 cells were rendered senescent by DXR treatment or retroviral infection of oncogenic ras (HRasV12), then subjected to RT-qPCR analysis for p16INK4a, SMS2 and nSMase2 gene expression (C) and western blotting (D). (E)–(I) Pre-senescent RPE-1 cells were treated with DXR and subjected to immunofluorescence staining for markers of DNA damage (γ-H2AX [red], pST/Q substrate [green] and DAPI [blue]) (E), RT-qPCR analysis (F) and to western blotting (G). The percentage of nuclei that contain more than 3 DNA damaging foci were shown in the histograms (E). NanoSight analysis of isolated sEV particles (H) and immuno-gold labelling for CD63, a well-known exosome marker, followed by transmission electron microscopy (TEM) (I). Scale bars, 10 μm. For all graphs, error bars indicate mean ± standard deviation (s.d.) of triplicate measurements. p values was calculated by unpaired two-tailed Student’s t-test (*** p < 0.001).
Figure 1. Gene expression associated with the ceramide synthetic pathway is changed by damage to DNA. (A,B) TIG-3 cells were treated with doxorubicin (DXR) for 48h and subjected to immunofluorescence staining for markers of DNA damage (γ-H2AX [red], phosphor-Ser/Thr ATM/ATR (pST/Q) substrate [green] and 40,6-diamidino-2-phenylindole: DAPI [blue]) (A) or to NanoSight analysis of isolated sEV particles (B). (C,D) Pre-senescent TIG-3 cells were rendered senescent by DXR treatment or retroviral infection of oncogenic ras (HRasV12), then subjected to RT-qPCR analysis for p16INK4a, SMS2 and nSMase2 gene expression (C) and western blotting (D). (E)–(I) Pre-senescent RPE-1 cells were treated with DXR and subjected to immunofluorescence staining for markers of DNA damage (γ-H2AX [red], pST/Q substrate [green] and DAPI [blue]) (E), RT-qPCR analysis (F) and to western blotting (G). The percentage of nuclei that contain more than 3 DNA damaging foci were shown in the histograms (E). NanoSight analysis of isolated sEV particles (H) and immuno-gold labelling for CD63, a well-known exosome marker, followed by transmission electron microscopy (TEM) (I). Scale bars, 10 μm. For all graphs, error bars indicate mean ± standard deviation (s.d.) of triplicate measurements. p values was calculated by unpaired two-tailed Student’s t-test (*** p < 0.001).
Ijms 21 03720 g001
Ijms 21 03720 g002 550
Figure 2. The ceramide pathway plays an important role in small EV secretion from HDFs. (A–C) After transfection with siRNA oligos against SMS2 twice, TIG-3 cells were then subjected to RT-qPCR analysis of SMS2 gene expression (A), western blotting (B), or to NanoSight analysis of isolated small EV particles (C). (D,E) After infection with retrovirus encoding FLAG-tagged SMS2 or empty vector and selection with puromycin, TIG-3 cells were treated with 150 nM DXR for 10 days and subjected to western blotting (D), or to NanoSight analysis of isolated small EV particles (E). (F–H) After transfection with siRNA oligos against nSMase2 twice, TIG-3 cells were subjected to RT-qPCR analysis of nSMase2 gene expression (F), western blotting (G), NanoSight analysis of isolated small EV particles (H), and to immunofluorescence staining for markers of DNA damage (γ-H2AX [red], pST/Q substrate [green] and DAPI [blue]) (I). The percentage of nuclei that contain more than 3 DNA damaging foci positive were shown in the histograms (I). (J,K) Pre-senescent TIG-3 cells were infected with retrovirus encoding FLAG-tagged nSMase2 or empty vector. After selection with puromycin, cells were subjected to western blotting (J), or to NanoSight analysis of isolated small EV particles (K). For all graphs, error bars indicate mean + standard deviation (s.d.) of triplicate measurements. P values was calculated by unpaired two-tailed Student’s t-test (** p < 0.01, *** p < 0.001).
Figure 2. The ceramide pathway plays an important role in small EV secretion from HDFs. (A–C) After transfection with siRNA oligos against SMS2 twice, TIG-3 cells were then subjected to RT-qPCR analysis of SMS2 gene expression (A), western blotting (B), or to NanoSight analysis of isolated small EV particles (C). (D,E) After infection with retrovirus encoding FLAG-tagged SMS2 or empty vector and selection with puromycin, TIG-3 cells were treated with 150 nM DXR for 10 days and subjected to western blotting (D), or to NanoSight analysis of isolated small EV particles (E). (F–H) After transfection with siRNA oligos against nSMase2 twice, TIG-3 cells were subjected to RT-qPCR analysis of nSMase2 gene expression (F), western blotting (G), NanoSight analysis of isolated small EV particles (H), and to immunofluorescence staining for markers of DNA damage (γ-H2AX [red], pST/Q substrate [green] and DAPI [blue]) (I). The percentage of nuclei that contain more than 3 DNA damaging foci positive were shown in the histograms (I). (J,K) Pre-senescent TIG-3 cells were infected with retrovirus encoding FLAG-tagged nSMase2 or empty vector. After selection with puromycin, cells were subjected to western blotting (J), or to NanoSight analysis of isolated small EV particles (K). For all graphs, error bars indicate mean + standard deviation (s.d.) of triplicate measurements. P values was calculated by unpaired two-tailed Student’s t-test (** p < 0.01, *** p < 0.001).
Ijms 21 03720 g002
Ijms 21 03720 g003 550
Figure 3. Inhibiting the ceramide pathway causes DNA damage accumulation in mice. (A–C) Mouse embryonic fibroblasts (MEFs) were treated with spiroepoxide and then subjected to NanoSight analysis of isolated small EV particles (A), cell proliferation analysis (B) or to immunofluorescence staining for markers of DNA damage (53BP1 [red] and DAPI [blue]) (C). Scale bars, 10 μm. The histograms indicate the percentage of nuclei that contain more than 3 foci positive for 53BP1 staining. At least 100 cells were scored per group (C). (D,E) ICR (CD1) mice were intraperitoneally injected with spiroepoxide every two days. After 14 days, the mice were euthanized and small intestines were subjected to NanoSight analysis (NTA) of isolated small EV particles (D) or to immunofluorescence analysis of intestine section (E). Section of intestines were subjected to immunofluorescence staining for markers of DNA damage (53BP1 [red] and DAPI [blue]) (E). The representative data from three independent experiments are shown. For all graphs, error bars indicate mean +standard deviation (s.d.) of triplicate measurements. p values was calculated by unpaired two-tailed Student’s t-test (* p < 0.05, ** p < 0.01, *** p < 0.001).
Figure 3. Inhibiting the ceramide pathway causes DNA damage accumulation in mice. (A–C) Mouse embryonic fibroblasts (MEFs) were treated with spiroepoxide and then subjected to NanoSight analysis of isolated small EV particles (A), cell proliferation analysis (B) or to immunofluorescence staining for markers of DNA damage (53BP1 [red] and DAPI [blue]) (C). Scale bars, 10 μm. The histograms indicate the percentage of nuclei that contain more than 3 foci positive for 53BP1 staining. At least 100 cells were scored per group (C). (D,E) ICR (CD1) mice were intraperitoneally injected with spiroepoxide every two days. After 14 days, the mice were euthanized and small intestines were subjected to NanoSight analysis (NTA) of isolated small EV particles (D) or to immunofluorescence analysis of intestine section (E). Section of intestines were subjected to immunofluorescence staining for markers of DNA damage (53BP1 [red] and DAPI [blue]) (E). The representative data from three independent experiments are shown. For all graphs, error bars indicate mean +standard deviation (s.d.) of triplicate measurements. p values was calculated by unpaired two-tailed Student’s t-test (* p < 0.05, ** p < 0.01, *** p < 0.001).
Ijms 21 03720 g003
Ijms 21 03720 g004 550
Figure 4. Inhibiting the autophagy pathway leads to the gene expression of SASP factors. (A,B) TIG-3 cells were treated with chloroquine (CQ) or bafilomycin A1 (BafA1) for 48 h and subjected to western blotting (A) and to cell proliferation analysis (B). (C–F) TIG-3 cells were treated with 20 μM Chloroquine or 10 nM bafilomycin A1 for 48 h and subjected to isolation of cytoplasmic fraction followed by qPCR analysis of chromosomal DNA in cytoplasm (C), RT-qPCR analysis of SASP factor gene expression (D), NanoSight analysis of isolated small EV particles (E) or to quantitative analysis of dsDNA in small EVs (F). (G) A model of the molecular mechanism. DNA damage activates the ceramide synthetic pathway, both through SMS2 downregulation and nSMase2 upregulation, blocking autophagy and promoting the release of small EVs. For all graphs, error bars indicate mean ± standard deviation (s.d.) of triplicate measurements. p values was calculated by unpaired two-tailed Student’s t-test (** p < 0.01, *** p < 0.001).
Figure 4. Inhibiting the autophagy pathway leads to the gene expression of SASP factors. (A,B) TIG-3 cells were treated with chloroquine (CQ) or bafilomycin A1 (BafA1) for 48 h and subjected to western blotting (A) and to cell proliferation analysis (B). (C–F) TIG-3 cells were treated with 20 μM Chloroquine or 10 nM bafilomycin A1 for 48 h and subjected to isolation of cytoplasmic fraction followed by qPCR analysis of chromosomal DNA in cytoplasm (C), RT-qPCR analysis of SASP factor gene expression (D), NanoSight analysis of isolated small EV particles (E) or to quantitative analysis of dsDNA in small EVs (F). (G) A model of the molecular mechanism. DNA damage activates the ceramide synthetic pathway, both through SMS2 downregulation and nSMase2 upregulation, blocking autophagy and promoting the release of small EVs. For all graphs, error bars indicate mean ± standard deviation (s.d.) of triplicate measurements. p values was calculated by unpaired two-tailed Student’s t-test (** p < 0.01, *** p < 0.001).
Ijms 21 03720 g004
Ijms 21 03720 g005 550
Figure 5. The release of small EVs blocks the inflammatory response caused by bacterial infection. (A) Timeline of the experimental procedure. (B–D) THP-1 cells were treated with 100 nM PMA for 7 days and transfected with indicated siRNA oligos. After incubation with Bacillus Calmette-Guérin (BCG), RT-qPCR analysis was performed for confirmation of knockdown efficiency (B) or innate immune responsible gene expression (C). The amounts of apoptotic cell death was quantitatively measured (D). For all graphs, error bars indicate mean +standard deviation (s.d.) of triplicate measurements. p values was calculated by unpaired two-tailed Student’s t-test (*** p < 0.001, N.S. (not significant)).
Figure 5. The release of small EVs blocks the inflammatory response caused by bacterial infection. (A) Timeline of the experimental procedure. (B–D) THP-1 cells were treated with 100 nM PMA for 7 days and transfected with indicated siRNA oligos. After incubation with Bacillus Calmette-Guérin (BCG), RT-qPCR analysis was performed for confirmation of knockdown efficiency (B) or innate immune responsible gene expression (C). The amounts of apoptotic cell death was quantitatively measured (D). For all graphs, error bars indicate mean +standard deviation (s.d.) of triplicate measurements. p values was calculated by unpaired two-tailed Student’s t-test (*** p < 0.001, N.S. (not significant)).
Ijms 21 03720 g005
Ijms 21 03720 g006 550
Figure 6. A model of our research. In healthy conditions, endogenous dsDNA fragments, derived from chromosomal or mitochondrial DNA, or exogenous dsDNA fragments, derived from bacterial or viral infection, are degraded by autophagy or released via small EVs. Therefore, these pathways function as defence mechanisms to prevent aberrant activation of innate immune responses. In senescent cells, irreparable DNA damage inhibits dsDNA degradation by autophagy and upregulates small EV secretion by activating the ceramide pathway. If neither pathway can function sufficiently, inflammasome activation occurs, leading to apoptosis. In summary, autophagy and the small EV pathway cooperatively play key roles to support cellular homeostasis.
Figure 6. A model of our research. In healthy conditions, endogenous dsDNA fragments, derived from chromosomal or mitochondrial DNA, or exogenous dsDNA fragments, derived from bacterial or viral infection, are degraded by autophagy or released via small EVs. Therefore, these pathways function as defence mechanisms to prevent aberrant activation of innate immune responses. In senescent cells, irreparable DNA damage inhibits dsDNA degradation by autophagy and upregulates small EV secretion by activating the ceramide pathway. If neither pathway can function sufficiently, inflammasome activation occurs, leading to apoptosis. In summary, autophagy and the small EV pathway cooperatively play key roles to support cellular homeostasis.
Ijms 21 03720 g006

Share and Cite

MDPI and ACS Style

Hitomi, K.; Okada, R.; Loo, T.M.; Miyata, K.; Nakamura, A.J.; Takahashi, A. DNA Damage Regulates Senescence-Associated Extracellular Vesicle Release via the Ceramide Pathway to Prevent Excessive Inflammatory Responses. Int. J. Mol. Sci. 2020, 21, 3720. https://doi.org/10.3390/ijms21103720

AMA Style

Hitomi K, Okada R, Loo TM, Miyata K, Nakamura AJ, Takahashi A. DNA Damage Regulates Senescence-Associated Extracellular Vesicle Release via the Ceramide Pathway to Prevent Excessive Inflammatory Responses. International Journal of Molecular Sciences. 2020; 21(10):3720. https://doi.org/10.3390/ijms21103720

Chicago/Turabian Style

Hitomi, Kazuhiro, Ryo Okada, Tze Mun Loo, Kenichi Miyata, Asako J. Nakamura, and Akiko Takahashi. 2020. "DNA Damage Regulates Senescence-Associated Extracellular Vesicle Release via the Ceramide Pathway to Prevent Excessive Inflammatory Responses" International Journal of Molecular Sciences 21, no. 10: 3720. https://doi.org/10.3390/ijms21103720

APA Style

Hitomi, K., Okada, R., Loo, T. M., Miyata, K., Nakamura, A. J., & Takahashi, A. (2020). DNA Damage Regulates Senescence-Associated Extracellular Vesicle Release via the Ceramide Pathway to Prevent Excessive Inflammatory Responses. International Journal of Molecular Sciences, 21(10), 3720. https://doi.org/10.3390/ijms21103720

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop