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Review

The Pathophysiological Significance of “Mitochondrial Ejection” from Cells

by
Qintao Fan
,
Yasuhiro Maejima
*,
Lai Wei
,
Shun Nakagama
,
Yuka Shiheido-Watanabe
and
Tetsuo Sasano
Department of Cardiovascular Medicine, Graduate School of Medical and Dental Sciences, Tokyo Medical and Dental University, Tokyo 113-8510, Japan
*
Author to whom correspondence should be addressed.
Biomolecules 2022, 12(12), 1770; https://doi.org/10.3390/biom12121770
Submission received: 4 November 2022 / Revised: 22 November 2022 / Accepted: 26 November 2022 / Published: 28 November 2022
(This article belongs to the Special Issue Advances in the Role of Mitochondria in Regulated Cell Death Dysfunctions Associated with Human Pathologies)
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Abstract

:
Mitochondria have beneficial effects on cells by producing ATP and contributing to various biosynthetic procedures. On the other hand, dysfunctional mitochondria have detrimental effects on cells by inducing cellular damage, inflammation, and causing apoptosis in response to various stimuli. Therefore, a series of mitochondrial quality control pathways are required for the physiological state of cells to be maintained. Recent research has provided solid evidence to support that mitochondria are ejected from cells for transcellular degradation or transferred to other cells as metabolic support or regulatory messengers. In this review, we summarize the current understanding of the regulation of mitochondrial transmigration across the plasma membranes and discuss the functional significance of this unexpected phenomenon, with an additional focus on the impact on the pathogenesis of cardiovascular diseases. We also provide some perspective concerning the unrevealed mechanisms underlying mitochondrial ejection as well as existing problems and challenges concerning the therapeutic application of mitochondrial ejection.

1. Introduction

Mitochondria are double membrane-bound α-proteobacterium-derived organelles that contain extrachromosomal deoxyribonucleic acid (DNA), termed mitochondrial DNA (mtDNA) [1]. Most of the genes that encode mitochondrial proteins have been transferred to the genome in the nucleus of host cells, with only 16 kilobases of circular DNA left in the mitochondria [2]. Mitochondria play a vital role by producing adenosine triphosphate (ATP), an essential energy source for all organisms. Concurrently with the adenosine triphosphate (ATP) generation, mitochondria are closely associated with other physiological metabolic pathways, including glycolysis, calcium homeostasis, steroid synthesis, and cell cycle regulation. On the other hand, mitochondria also participate in a series of pathological processes [3]. Reactive oxygen species (ROS), which cause damage to proteins, nucleic acids, and lipids in the host cells, are produced as byproducts of the OXPHOS process [4]. As a result of mitochondrial damage, mtDNA can be released, thereby playing a detrimental role by triggering various proinflammatory signaling pathways [5,6]. A series of mitochondrial quality control systems, namely the ubiquitin-proteasome system (UPS), mitochondrial dynamics, and mitochondria-selective autophagy (mitophagy) remove damaged mitochondrial components [7,8,9,10]. As cardiomyocytes (CMs) are post-mitotic cells that require long-term survival, it is essential to maintain tight control over the quality of mitochondria. Thus, impairment of the mitochondrial quality control systems provokes critical cardiovascular diseases, including heart failure [11,12,13].
Recent investigations have revealed that unexpected mechanisms are involved in maintaining mitochondrial quality in cells by transporting mitochondria between the inside and outside of cells and across plasma membranes. For example, it has been shown that nerve cells, CMs, and adipocytes are able to eject damaged mitochondria from their cytosol [14,15,16]. Macrophages have dual roles in the uptake and elimination of mitochondria. Stem cells are able to donate healthy mitochondria that can enhance the aerobic respiration capacity of recipient cells [17]. In addition, mitocytosis, a special mitochondrial quality control process through which damaged mitochondria are transported into migrasomes for the disposal of them from migrating cells, has recently been reported [18]. In this review, we summarize the current understanding of the regulation of mitochondrial transmigration across plasma membranes and discuss the functional significance of this unexpected phenomenon, with a focus on the impact on the pathogenesis of cardiovascular diseases.

2. Disposal and Elimination of Damaged Mitochondria

In 2014, Davis et al. detected transcellular mitochondrial degradation from retinal ganglion cell axons to astrocytes under baseline conditions in vivo [19]. Using three-dimensional electron microscopy (EM), they identified axonal evulsions that contained mitochondria surrounded by astrocytes, and transmission EM revealed the presence of both intact mitochondrial structures and irregular mitochondria-like membranous bodies. Mitochondria shed into evulsions were taken and eliminated by adjacent astrocytes. These results implied that a similar process occurs in the murine cerebral cortex. A recent study demonstrated that damaged mitochondria were released from neurons to culture media [15]. The number of depolarized mitochondria released from the cytosol to extracellular spaces was markedly increased by treatment with rotenone or carbonyl cyanide m-chlorophenylhydrazone (CCCP), the inducers of mitochondrial stress, in PC12 cells [15]. The overexpression of Parkin (PRKN), a mitophagy regulator that is associated with hereditary Parkinson’s disease, or PRKN-independent regulators reduced the release of mitochondria [15]. On the other hand, the number of ejected mitochondria was markedly increased in autophagy-deficient cells [15]. Additionally, it has been shown that the number of mitochondria released into media was enhanced by acidotic conditions (the cells were incubated with pH6.5 solution) or oxidant-induced stress in mouse primary neurons [20]. Falchi et al. found that ejected mitochondria from human-cultured fetal astrocytes in large vesicles (1–8 μm) were eliminated by phagocytic cells with undetermined mechanisms [21].
According to a report by Melentijevic et al., the ejection of injured mitochondria occurred in a Caenorhabditis elegans (C. elegans) model [22]. The neurons of C. elegans eject “exophers”, membranous vesicles of 2–15 μm in diameter which contain mitochondria and other organelles or proteins. The production of exophers is provoked by various stresses, the suppression of autophagy or UPS activities, and mitochondrial damage. Recently, Nicolás-Ávila et al. revealed a transcellular mitochondrial degradation pathway between CMs and macrophages in healthy myocardium [14]. They found that CMs packed damaged mitochondria in LC3+ exophers for ejection to extracellular spaces in baseline, and isoproterenol-induced cardiac stress promoted the ejection of exophers (Figure 1A). Released exophers were phagocytized and degraded by cardiac-resident macrophages (cMacs). Such a phenomenon is termed “Heterophagy” [23]. Both the stimulation and suppression of autophagy could induce a parallel trend in the release of exopher, suggesting that the exopher-mediated disposal system of mitochondria would be controlled by autophagy-associated regulators [23] (Figure 1A). In accordance with apoptotic cells, phosphatidyl serine, an “eat-me” signal that is recognized by MER proto-oncogene tyrosine kinase (MERTK)—a type of tyrosine kinase that is highly expressed in cMacs—was found to be expressed on the surface of exophers. MERTK deletion caused the removal of exophers to become stuck, suggesting that MERTK would be a receptor of exophers in cMacs [23]. In addition, the ablation of cMacs caused the accumulation of exophers, which resulted in the provocation of cardiac inflammation, suggesting that the release of exophers plays a critical role in maintaining a healthy condition in the heart [23].
Rosina et al. revealed that the transcellular degradation of damaged mitochondria between brown adipocytes and brown adipose tissue (BAT)-resident macrophages was mediated through extracellular vesicles (EVs) [16]. Under cold stress, brown adipocytes eject oxidatively-injured mitochondria via EVs, which diminish the mitochondrial function after their re-uptake by other brown adipocytes. The clearance of these EVs is executed by BAT-resident macrophages. The in vivo depletion of macrophages resulted in the accumulation of mitochondria-containing EVs and, subsequently, in impaired thermogenesis in BAT, suggesting the importance of this process in maintaining thermogenic homeostasis in BATs [16]. This study differs from the previous findings of Crewe et al. since EVs containing functional but damaged mitochondria, which were produced by stressed adipocytes, were found to enter isolated CMs, thereby promoting the production of ROS while also having a compensatory antioxidant effect in the heart [24].
Mitocytosis is a migrasome-mediated mitochondrial disposal process that is regarded as a crucial mitochondrial quality control system in migrating cells [18]. When cells start migrating, tubular structures termed “retraction fibers” grow from the end of the tail. In the next step of cell migration, cellular components are transferred, thereby accumulating in retraction fibers. Then, accumulated cellular components form large vesicular organelles called “migrasomes”. Finally, when the cells move away, migrasomes are left behind or taken up by adjacent cells [25] (Figure 1B). Jiao et al. found the existence of mitochondria with clearly visible cristae-like structures in migrasomes induced by CCCP-treated L929 cells [18]. Time-lapse imaging enabled them to observe that tubular-form mitochondria were transported outward with extension in a highly dynamic manner [25]. Part of the mitochondria that moved to the peripheral area of the cells appeared to be separated from the mitochondrial network and was captured in the plasma membrane, and was thereby transferred into migrasomes wherein the host cells migrate away. Intriguingly, damaged mitochondria—as evidenced by decreased membrane potential with a high ROS production—are selectively transported to the peripheral area of cells, and are thereby released into migrasomes [25]. Damaged mitochondria have a weakened ability to rescue dynein, the inward motor, while their ability to bind kinesin family member 5B (KIF5B) significantly increased. Therefore, in cooperation with mitochondrial fission regulator dynamin-related protein 1 (Drp1) and myosin XIX (Myo19), damaged mitochondria are transferred to the peripheral area of cells and then are disposed of by migrasomes [25] (Figure 1B). Thus, the mitocytosis-mediated mitochondrial disposal process plays a critical role in the maintenance of mitochondrial quality and intracellular homeostasis.

3. Role of Released Mitochondria as a “Savior” of Target Cells

The intercellular transport of mitochondria was first reported by Koyanagi et al. in 2005 [26]. A subsequent study demonstrated the importance of mitochondrial transfer in vitro which improved the aerobic respiration of mtRNA-depleted recipient cells [27]. Accumulating lines of evidence suggest that mesenchymal stem cells (MSCs) play a role in the protection of various other cells by providing their intact mitochondria to other damaged cells via intercellular mitochondrial transportation. For instance, MSCs have the ability to rescue CMs from ischemia-induced damage via mitochondrial transportation, which is mediated through tunneling nanotubes [28,29]. Mitochondria—but not cytoplasm—could be exclusively transferred toward CMs [30]. O’Brien et al. demonstrated that MSCs were able to transport mitochondria through large EVs to doxorubicin-treated patient-specific induced pluripotent stem cell-derived CMs (iCMs), thereby improving contractility and the mitochondrial function of acceptor cells [31].
It has been shown that MSCs alleviated airway epithelial cells from lipopolysaccharide (LPS)-induced acute lung injury [32] and asthma inflammation [33] by providing intact mitochondria to damaged cells. Similarly, Li et al. revealed that transplanted induced pluripotent stem cells (iPSC)-MSCs rescued airway epithelial cells from cigarette smoke-induced damage via the transference of mitochondria [34]. The salutary roles of mitochondrial transfer from MSCs to neurons have been detected. Transferred mitochondria from MSCs were able to repair the respiration of recipient neurons, thereby reducing the ischemic damage [35] or oxidant injury [36] of damaged neurons. Further research demonstrated the ability of MSCs to transfer mitochondria to astrocytes [37] and neural stem cells [38] for exerting a protective effect on the recipient cells.
Recent investigations revealed that the intercellular transport of mitochondria could also be seen between mature cells. Astrocytes transport mitochondria to neurons to protect the neuronal function in response to transient focal cerebral ischemia in mice [39] and cisplatin-treated cultured neurons [40]. Mitochondria are able to vigorously transfer between neurons and astrocytes [41] or brain endothelial cells and neurons [42]. Similarly, Shen et al. reported that mitochondrial transfer between neonatal rat CMs and cardiac myofibroblasts (MFs) protected CMs from damage-induced apoptosis [43,44]. A recent report demonstrated that human iCMs are able to produce mitochondria-containing EVs. The intramyocardial injection of mitochondria-containing EVs isolated from the culture media of iCMs relieved cardiac dysfunction in the murine post-infarction heart failure model, suggesting that the transplantation of mitochondria-containing EVs to the CMs could be a potential novel therapeutic strategy for post-infarction heart failure [45]. Mitochondrial transport between matured cells also occurs in the kidneys [46] and osseous tissue [47], where it restores the metabolic function of recipient cells.
The intercellular transport of mitochondria is also involved in the genesis, survival, metastatic transformation, and drug resistance of malignant tumors [48]. Thus far, mitochondrial transportation has been observed in breast cancer, lung cancer, melanoma, and leukemia. It has been shown that malignant cells receive mitochondria from non-malignant cells to restore their respiratory function [49,50] and/or acquire chemoresistance [49,51,52]. Recently, Saha et al. demonstrated an intriguing phenomenon wherein cancer cells “hijack” mitochondria from immune cells by sucking through nanotubes, thereby improving their own metabolic activity and causing immune cell death [53].

4. Released Mitochondria-Mediated Regulation of the Immune System

It is widely recognized that mitochondria exert an immunomodulatory function through various mechanisms. The metabolic activities and metabolites of mitochondria are related to the regulation of immune activities of various immune cells. Similarly, mtDNA is closely associated with immunoreaction as a damage-associated molecular pattern (DAMP). Recently, immunoregulation mediated by “intercellular mitochondrial transfer” has received attention. Boudreau et al. substantiated the existence of functional mitochondria in EVs released by platelets, which was found in platelet concentrates used for transfusion [54]. They also found that the hydrolysis of such extracellular mitochondria leads to the release of phospholipase A2 IIA (sPLA2-IIA), which results in the promotion of inflammation. Two-photon microscopy revealed that extracellular mitochondria triggered the adhesion of neutrophils, suggesting that extracellular mitochondria play an important role in the initiation of inflammatory responses. Puhm et al. demonstrated that monocytes could release mitochondria-contained EVs in response to LPS-mediated activation [55]. They also revealed that any mitochondria directly isolated from LPS-activated monocytes, mitochondria-containing EVs isolated from monocytes, and circulating EVs isolated from volunteers receiving low-dose LPS injections could provoke type I Interferon (IFN) and tumor necrosis factor (TNF) responses in endothelial cells. On the other hand, the loss of mitochondrial respiratory capacity, the presence of pyruvate, and MitoTEMPO, a mitochondrial reactive oxygen species scavenger, dramatically reduced the inflammatory response. Hough et al. reported that mitochondria-containing EVs could be seen in the bronchoalveolar lavage fluid of both healthy volunteers and asthmatics [56]. Although it is possible that those mitochondria-containing EVs were released from airway myeloid-derived regulatory cells and internalized by recipient T cells, their functions remain unclear.
A growing body of evidence suggests that mitochondrial transport by MSCs plays an important role in the regulation of immune responses. In an animal model of acute respiratory distress syndrome (ARDS), MSCs assisted the removal of bacteria by transferring mitochondria to macrophages via tunneling nanotubes (TNTs) [57] or mitochondria-containing EVs [58]. Mitochondrial transport could induce the differentiation of macrophages to the anti-inflammatory M2 phenotype with enhanced phagocytosis ability, thereby reducing the inflammatory response [58,59]. In the case of primary CD4+CCR6+CD45RO+ T helper 17 (Th17) cells cocultured with MSCs, transported mitochondria from MSCs caused interconversion of Th17 cells into T regulatory cells, which resulted in the significant impairment of IL-17 production from Th17 cells [60]. A subsequent investigation demonstrated that MSC-derived mitochondria enhanced the expression of FOXP3, IL2RA, CTLA4, and TGFβ1 in CD4+ T cells, thereby promoting the activation of T-cells or differentiation into regulatory T cells. Indeed, the transplantation of MSC-derived mitochondria-treated CD4+ T cells significantly reduced the organ damage caused by inflammation and improved the survival rate in murine graft-versus-host disease models [61]. In addition, it has been shown that MSC-derived mitochondria play a suppressive role in the activity of autophagy in T cells, thereby inhibiting the apoptosis of T cells caused by high autophagy activity [62].

5. Mechanisms of Mitochondrial Release/Transfer from Cells

Although numerous studies have revealed several routes of mitochondrial release/transfer, including TNTs and MVs, the specific molecular mechanisms remain to be elucidated. In this article, we have summarized the current understanding of the molecular mechanisms involved in the mitochondrial release and/or transfer from cells (Table 1).
TNTs, a unique intercellular membrane structure, were first reported in rat pheochromocytoma PC12 cells [70]. TNTs have a diameter of 50–200 nm, which allows the transport of cell membranes, plasma, and organelles, such as mitochondria, between cells through intercellular connected tubes (Figure 2A). A variety of stimuli that cause mitochondrial damage can induce the formation of TNTs. Mechanistically, p53 is considered to be an important upstream regulator in the process of TNT formation [71]. Activated p53 triggers the epidermal growth factor receptor activation, followed by the upregulation of the downstream Akt-phosphatidylinositol-3 kinase-mTOR pathway, leading to the high expression of M-sec (TNFαIP2). M-sec is one of the key regulators in the formation of TNTs [72], which is responsible for mediating the assembly of exocyst complexes by interacting with RalA to induce F-actin polymerization. CD38, a transmembrane glycoprotein known as cyclic ADP ribose hydrolase, is expected to be a key regulator of TNT-mediated mitochondrial transfer. In the co-culture model of primary multiple myeloma cells and BMSC, TNT-mediated mitochondrial transfer to multiple myeloma cells is inhibited by the shRNA-mediated knockdown of CD38 [49]. Wang et al. demonstrated that enhanced CD38 expression caused by the activation of extracellular regulated protein kinases 1/2 (ERK1/2) promoted mitochondrial transfer from astrocytes [73]. The intercellular concentration gradient of the S100 calcium-binding protein A4 (S100A4) is known to be closely associated with the process of TNT elongation. Namely, a previous report demonstrated that TNTs expand from the donor cells with lower concentrations of S100A4 to receptor cells with higher concentrations [74]. In addition, Cdc42 has been suggested to be involved in the prolongation of TNTs [72]. Gap junction protein connexin 43 (CX43) mediates mitochondrial transfer between bone marrow-derived stem cells and LPS-damaged alveolar epithelial cells [32], possibly through the promotion of TNT formation [33]. On the other hand, He et al. demonstrated that CX43 is absent in the TNTs between neonatal rat CMs and cardiac fibroblasts (CFs) [43], suggesting that further studies are needed to determine the specific role of CX43 in the formation of TNTs. Recent studies have revealed that Miro1, a mitochondrial outer membrane protein, plays an important role in regulating the intercellular movement of mitochondria along TNTs [36,37,68,69]. As Miro1 is a type of calcium-sensitive Rho-GTPase [75], it can be bound to TRAK1/2, which results in the mediation of the movement of mitochondria by recruiting a series of kinesins. In addition, Miro1 interacts with mitofusins (Mfn1 and Mfn2), thereby facilitating the transport of mitochondria along TNTs [76]. Shen et al. demonstrated that mitochondrial transport along TNTs is mediated by KIF5B, a member of the kinesin superfamily, in the co-culture system of neonatal rat CMs and CFs [44].
EV is another important transporter of mitochondria (Figure 2B). EVs are membranous structures derived from the endosomal system or shed from the plasma membrane, including exosomes and microvesicles, which differ in size and origin [77]. Previous studies have shown that cells can secrete EVs with mitochondrial components. Although the molecular mechanism needs to be further elucidated, a potential link between the mitochondria-containing EV and the mitochondrial-derived vesicle (MDV), a unique vesicle capable of transporting mitochondria to other organelles has been revealed [16,24,78]. MDVs are generated through the selective packing of mitochondrial content and transported to lysosomes to be degraded early on in mitochondrial damage, causing them to be considered an early response of mitochondrial quality control [79]. A recent study demonstrated that the packaging of mitochondrial proteins into EVs requires the expression of Snx9 and OPA1, while PRKN facilitates the delivery of MDVs containing damaged mitochondrial components to lysosomes rather than EVs, thus preventing the release of mitochondrial DAMPs [78]. Consistently, the inhibition of lysosomal activity promotes the release of mitochondria containing EVs in adipocytes [16,24]. However, according to previous studies, oxidatively damaged mitochondrial proteins are enriched in both MDVs and EVs isolated from stressed adipocytes, suggesting some dysfunction in the selective packaging process.
In addition to participating in TNT-mediated mitochondrial transfer, CD38 is involved in the extracellular release of mitochondrial particles by astrocytes [39]. As mentioned above, astrocytes promote the survival of neurons by producing mitochondrial EVs after a stroke, while the inhibition of CD38 was shown to significantly decrease the number of mitochondria containing EVs, suggesting that a CD38-dependent pathway is required for the ejection of these EVs.
Mitochondria can be ejected from cells or transferred to other cells through various other pathways. Activated platelets release functional mitochondria through the actin-dependent pathway, which is independent of the microtubule-dependent pathway. This process is considered to be a damage-associated mechanism [54]. LPS-treated monocytic cells extrude naked mitochondria with uncertain molecular mechanisms [55].

6. Concluding Remarks

In summary, we reviewed the functional significance of mitochondrial transmigration across the plasma membranes in various cells. We also summarized the trends in investigations of such phenomena as novel therapeutic targets of various diseases, including heart failure. In recent years, mitochondrial supplemental therapy—based on mitochondrial transfer—has been proven to improve the function of various damaged tissues and organs. Previous studies have verified the potential efficacy of MSC transplantation-mediated mitochondrial supplemental therapy in animal experiments [69,80]. With the emergence of new technologies, the focus of mitochondrial transfer therapeutics is gradually shifting from cell-dependent therapy to cell-free therapy. Indeed, EV-based mitochondrial transplantation has been shown to be capable of significantly improving the function of ischemic myocardium after treatment, and it is favored due to its stability in stressed environments [45]. However, there are several critical limitations to these therapeutic strategies. For example, considering that the mechanism of selectivity of mitochondrial transfer to recipient cells remains unclear, the safety issues caused by undesired transfer and its potential effects (unwanted redifferentiation, excess mitochondria, ATP in recipient cells, etc.) need to be further elucidated. In addition, although studies on mitochondrial transfer have been extensively conducted in the fields of immunology, cancer biology, and neuroscience, very few studies on mitochondrial transfer have been conducted in the field of cardiovascular science. As mitochondrial transfer therapy is expected to have great therapeutic potential in cardiovascular diseases, more attention is needed.
Increasing lines of evidence suggest that the ejection of damaged mitochondria plays an important role in maintaining the quality of intracellular mitochondria. However, our understanding of the molecular mechanisms involved in the regulation of such a process remains limited. Recent studies have shown that MDVs are involved in the extracellular ejection of damaged mitochondria via EVs [16,24]. However, the mechanism by which these EVs are transported outward and finally released is still poorly understood. For instance, the mechanism underlying the release of exophers from cells is completely unknown. The process through which damaged mitochondria are ejected remains unclear, but possible mechanisms include selective packing into MDV-like vesicles or autophagosomes before ejection into extracellular spaces or direct transportation via a mitocytosis-like process. Furthermore, we still know very little about how extracellular emissions and the intracellular mitochondrial quality control system share roles in the removal of damaged mitochondria. Cardiomyocytes rely heavily on mitochondrial quality control mechanisms to maintain their survival and cell function. Due to their huge energy demands and massive amounts of mitochondria, additional mechanics, such as the ejection of exophers, may be required to cope with stress and damage. Indeed, 60% of total mitochondria in healthy myocardium are ejected through exophers [14], a percentage that increases even further in response to stress, suggesting that this mechanism may be more adaptable than intracellular mitochondrial quality control mechanisms, including mitophagy, and act as a unique countermeasure to injury in cardiomyocytes (Figure 3). In addition, the expression of LC3 on the surface of exophers, together with the effect of autophagy regulation on the number of exophers, suggests that this mechanism is associated with autophagy machinery. The solution to these unsolved questions will help us to further understand the association between the release of damaged mitochondria and the pathogenesis of cardiovascular diseases, and ultimately promote the application of mitochondrial transplantation therapy for these conditions.

Author Contributions

Q.F. and Y.M. wrote the manuscript, and the authors reviewed and approved the manuscript for publication. L.W. drew illustrations for all figures in this manuscript. S.N. and Y.S.-W. participated in the research project on mitochondrial quality control in the heart and conducted a critical reading of the manuscript. T.S. supervised and appraised the manuscript. All authors have read and agreed to the published version of the manuscript.

Funding

This work was supported by a grant from Boehringer Ingelheim, JSPS KAKENHI Grant-in-Aid for Scientific Research (C) (20K08399 to Yasuhiro Maejima).

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

Not applicable.

Acknowledgments

We would like to thank Brian Quinn for English language editing.

Conflicts of Interest

The authors declare no conflict of interest in association with the present study.

References

  1. Friedman, J.R.; Nunnari, J. Mitochondrial form and function. Nature 2014, 505, 335–343. [Google Scholar] [CrossRef] [Green Version]
  2. Gabaldon, T.; Huynen, M.A. Shaping the mitochondrial proteome. Biochim. Biophys. Acta (BBA)-Bioenerg. 2004, 1659, 212–220. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  3. Nunnari, J.; Suomalainen, A. Mitochondria: In Sickness and in Health. CELL 2012, 148, 1145–1159. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  4. Chance, B.; Sies, H.; Boveris, A. Hydroperoxide metabolism in mammalian organs. Physiol. Rev. 1979, 59, 527–605. [Google Scholar] [CrossRef]
  5. West, A.P.; Shadel, G.S. Mitochondrial DNA in innate immune responses and inflammatory pathology. Nat. Rev. Immunol. 2017, 17, 363–375. [Google Scholar] [CrossRef]
  6. Yamazoe, M.; Sasano, T.; Ihara, K.; Takahashi, K.; Nakamura, W.; Takahashi, N.; Komuro, H.; Hamada, S.; Furukawa, T. Sparsely methylated mitochondrial cell free DNA released from cardiomyocytes contributes to systemic inflammatory response accompanied by atrial fibrillation. Sci. Rep. 2021, 11, 5837. [Google Scholar] [CrossRef] [PubMed]
  7. Ni, H.; Williams, J.A.; Ding, W. Mitochondrial dynamics and mitochondrial quality control. Redox Biol. 2015, 4, 6–13. [Google Scholar] [CrossRef] [Green Version]
  8. Sciarretta, S.; Maejima, Y.; Zablocki, D.; Sadoshima, J. The Role of Autophagy in the Heart. Annu. Rev. Physiol. 2018, 80, 1–26. [Google Scholar] [CrossRef] [PubMed]
  9. Bragoszewski, P.; Turek, M.; Chacinska, A. Control of mitochondrial biogenesis and function by the ubiquitin–proteasome system. Open Biol. 2017, 7, 170007. [Google Scholar] [CrossRef] [Green Version]
  10. Song, J.; Herrmann, J.M.; Becker, T. Quality control of the mitochondrial proteome. Nat. Rev. Mol. Cell Biol. 2021, 22, 54–70. [Google Scholar] [CrossRef]
  11. Picca, A.; Mankowski, R.T.; Burman, J.L.; Donisi, L.; Kim, J.; Marzetti, E.; Leeuwenburgh, C. Mitochondrial quality control mechanisms as molecular targets in cardiac ageing. Nat. Rev. Cardiol. 2018, 15, 543–554. [Google Scholar] [CrossRef] [PubMed]
  12. Rosca, M.G.; Hoppel, C.L. Mitochondrial dysfunction in heart failure. Heart Fail. Rev. 2012, 18, 607–622. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  13. Tahrir, F.G.; Langford, D.; Amini, S.; Mohseni Ahooyi, T.; Khalili, K. Mitochondrial quality control in cardiac cells: Mechanisms and role in cardiac cell injury and disease. J. Cell. Physiol. 2019, 234, 8122–8133. [Google Scholar] [CrossRef]
  14. Nicolás-Ávila, J.A.; Lechuga-Vieco, A.V.; Esteban-Martínez, L.; Sánchez-Díaz, M.; Díaz-García, E.; Santiago, D.J.; Rubio-Ponce, A.; Li, J.L.; Balachander, A.; Quintana, J.A.; et al. A Network of Macrophages Supports Mitochondrial Homeostasis in the Heart. Cell 2020, 183, 94–109.e23. [Google Scholar] [CrossRef]
  15. Choong, C.; Okuno, T.; Ikenaka, K.; Baba, K.; Hayakawa, H.; Koike, M.; Yokota, M.; Doi, J.; Kakuda, K.; Takeuchi, T.; et al. Alternative mitochondrial quality control mediated by extracellular release. Autophagy 2021, 17, 2962–2974. [Google Scholar] [CrossRef]
  16. Rosina, M.; Ceci, V.; Turchi, R.; Chuan, L.; Borcherding, N.; Sciarretta, F.; Sánchez-Díaz, M.; Tortolici, F.; Karlinsey, K.; Chiurchiù, V.; et al. Ejection of damaged mitochondria and their removal by macrophages ensure efficient thermogenesis in brown adipose tissue. Cell Metab. 2022, 34, 533–548.e12. [Google Scholar] [CrossRef] [PubMed]
  17. Liu, D.; Gao, Y.; Liu, J.; Huang, Y.; Yin, J.; Feng, Y.; Shi, L.; Meloni, B.P.; Zhang, C.; Zheng, M.; et al. Intercellular mitochondrial transfer as a means of tissue revitalization. Signal Transduct. Target. Ther. 2021, 6, 65. [Google Scholar] [CrossRef]
  18. Jiao, H.; Jiang, D.; Hu, X.; Du, W.; Ji, L.; Yang, Y.; Li, X.; Sho, T.; Wang, X.; Li, Y.; et al. Mitocytosis, a migrasome-mediated mitochondrial quality-control process. Cell 2021, 184, 2896–2910.e13. [Google Scholar] [CrossRef] [PubMed]
  19. Davis, C.O.; Kim, K.; Bushong, E.A.; Mills, E.A.; Boassa, D.; Shih, T.; Kinebuchi, M.; Phan, S.; Zhou, Y.; Bihlmeyer, N.A.; et al. Transcellular degradation of axonal mitochondria. Proc. Natl. Acad. Sci. USA 2014, 111, 9633–9638. [Google Scholar] [CrossRef] [Green Version]
  20. Gao, L.; Liu, F.; Hou, P.; Manaenko, A.; Xiao, Z.; Wang, F.; Xu, T.; Hu, Q. Neurons Release Injured Mitochondria as “Help-Me” Signaling After Ischemic Stroke. Front. Aging Neurosci. 2022, 14, 785761. [Google Scholar] [CrossRef]
  21. Falchi, A.M.; Sogos, V.; Saba, F.; Piras, M.; Congiu, T.; Piludu, M. Astrocytes shed large membrane vesicles that contain mitochondria, lipid droplets and ATP. Histochem. Cell Biol. 2012, 139, 221–231. [Google Scholar] [CrossRef] [PubMed]
  22. Melentijevic, I.; Toth, M.L.; Arnold, M.L.; Guasp, R.J.; Harinath, G.; Nguyen, K.C.; Taub, D.; Parker, J.A.; Neri, C.; Gabel, C.V.; et al. elegans neurons jettison protein aggregates and mitochondria under neurotoxic stress. Nature 2017, 542, 367–371. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  23. Nicolás-Ávila, J.A.; Pena-Couso, L.; Muñoz-Cánoves, P.; Hidalgo, A. Macrophages, Metabolism and Heterophagy in the Heart. Circ. Res. 2022, 130, 418–431. [Google Scholar] [CrossRef]
  24. Crewe, C.; Funcke, J.; Li, S.; Joffin, N.; Gliniak, C.M.; Ghaben, A.L.; An, Y.A.; Sadek, H.A.; Gordillo, R.; Akgul, Y.; et al. Extracellular vesicle-based interorgan transport of mitochondria from energetically stressed adipocytes. Cell Metab. 2021, 33, 1853–1868.e11. [Google Scholar] [CrossRef] [PubMed]
  25. Ma, L.; Li, Y.; Peng, J.; Wu, D.; Zhao, X.; Cui, Y.; Chen, L.; Yan, X.; Du, Y.; Yu, L. Discovery of the migrasome, an organelle mediating release of cytoplasmic contents during cell migration. Cell Res. 2015, 25, 24–38. [Google Scholar] [CrossRef] [Green Version]
  26. Koyanagi, M.; Brandes, R.P.; Haendeler, J.; Zeiher, A.M.; Dimmeler, S. Cell-to-Cell Connection of Endothelial Progenitor Cells with Cardiac Myocytes by Nanotubes: A Novel Mechanism for Cell Fate Changes? Circ. Res. 2005, 96, 1039–1041. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  27. Spees, J.L.; Olson, S.D.; Whitney, M.J.; Prockop, D.J. Mitochondrial Transfer between Cells Can Rescue Aerobic Respiration. Proc. Natl. Acad. Sci. USA 2006, 103, 1283–1288. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  28. Cselenyák, A.; Pankotai, E.; Horváth, E.M.; Kiss, L.; Lacza, Z. Mesenchymal stem cells rescue cardiomyoblasts from cell death in an in vitro ischemia model via direct cell-to-cell connections. BMC Cell Biol. 2010, 11, 29. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  29. Han, H.; Hu, J.; Yan, Q.; Zhu, J.; Zhu, Z.; Chen, Y.; Sun, J.; Zhang, R. Bone marrow-derived mesenchymal stem cells rescue injured H9c2 cells via transferring intact mitochondria through tunneling nanotubes in an in vitro simulated ischemia/reperfusion model. Mol. Med. Rep. 2016, 13, 1517–1524. [Google Scholar] [CrossRef] [Green Version]
  30. Plotnikov, E.Y.; Khryapenkova, T.G.; Vasileva, A.K.; Marey, M.V.; Galkina, S.I.; Isaev, N.K.; Sheval, E.V.; Polyakov, V.Y.; Sukhikh, G.T.; Zorov, D.B. Cell-to-cell cross-talk between mesenchymal stem cells and cardiomyocytes in co-culture. J. Cell. Mol. Med. 2008, 12, 1622–1631. [Google Scholar] [CrossRef]
  31. O’Brien, C.G.; Ozen, M.O.; Ikeda, G.; Vaskova, E.; Jung, J.H.; Bayardo, N.; Santoso, M.R.; Shi, L.; Wahlquist, C.; Jiang, Z.; et al. Mitochondria-Rich Extracellular Vesicles Rescue Patient-Specific Cardiomyocytes from Doxorubicin Injury: Insights Into the SENECA Trial. JACC CardioOncol. 2021, 3, 428–440. [Google Scholar] [CrossRef] [PubMed]
  32. Islam, M.N.; Das, S.R.; Emin, M.T.; Wei, M.; Sun, L.; Westphalen, K.; Rowlands, D.J.; Quadri, S.K.; Bhattacharya, S.; Bhattacharya, J. Mitochondrial transfer from bone-marrow-derived stromal cells to pulmonary alveoli protects against acute lung injury. Nat. Med. 2012, 18, 759–765. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  33. Yao, Y.; Fan, X.; Jiang, D.; Zhang, Y.; Li, X.; Xu, Z.; Fang, S.; Chiu, S.; Tse, H.; Lian, Q.; et al. Connexin 43-Mediated Mitochondrial Transfer of iPSC-MSCs Alleviates Asthma Inflammation. Stem Cell Rep. 2018, 11, 1120–1135. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  34. Li, X.; Zhang, Y.; Yeung, S.C.; Liang, Y.; Liang, X.; Ding, Y.; Ip, M.S.M.; Tse, H.; Mak, J.C.W.; Lian, Q. Mitochondrial transfer of induced pluripotent stem cell-derived mesenchymal stem cells to airway epithelial cells attenuates cigarette smoke-induced damage. Am. J. Respir. Cell Mol. Biol. 2014, 51, 455–465. [Google Scholar] [CrossRef]
  35. Babenko, V.A.; Silachev, D.N.; Zorova, L.D.; Pevzner, I.B.; Khutornenko, A.A.; Plotnikov, E.Y.; Sukhikh, G.T.; Zorov, D.B. Improving the Post-Stroke Therapeutic Potency of Mesenchymal Multipotent Stromal Cells by Cocultivation With Cortical Neurons: The Role of Crosstalk Between Cells. Stem Cells Transl. Med. 2015, 4, 1011–1020. [Google Scholar] [CrossRef]
  36. Tseng, N.; Lambie, S.C.; Huynh, C.Q.; Sanford, B.; Patel, M.; Herson, P.S.; Ormond, D.R. Mitochondrial transfer from mesenchymal stem cells improves neuronal metabolism after oxidant injury in vitro: The role of Miro1. J. Cereb. Blood Flow Metab. 2021, 41, 761–770. [Google Scholar] [CrossRef]
  37. Babenko, V.A.; Silachev, D.N.; Popkov, V.A.; Zorova, L.D.; Pevzner, I.B.; Plotnikov, E.Y.; Sukhikh, G.T.; Zorov, D.B. Miro1 Enhances Mitochondria Transfer from Multipotent Mesenchymal Stem Cells (MMSC) to Neural Cells and Improves the Efficacy of Cell Recovery. Molecules 2018, 23, 687. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  38. Boukelmoune, N.; Chiu, G.S.; Kavelaars, A.; Heijnen, C.J. Mitochondrial transfer from mesenchymal stem cells to neural stem cells protects against the neurotoxic effects of cisplatin. Acta Neuropathol. Commun. 2018, 6, 139. [Google Scholar] [CrossRef]
  39. Hayakawa, K.; Esposito, E.; Wang, X.; Terasaki, Y.; Liu, Y.; Xing, C.; Ji, X.; Lo, E.H. Transfer of mitochondria from astrocytes to neurons after stroke. Nature 2016, 535, 551–555. [Google Scholar] [CrossRef] [Green Version]
  40. English, K.; Shepherd, A.; Uzor, N.; Trinh, R.; Kavelaars, A.; Heijnen, C.J. Astrocytes rescue neuronal health after cisplatin treatment through mitochondrial transfer. Acta Neuropathol. Commun. 2020, 8, 36. [Google Scholar] [CrossRef]
  41. Gao, L.; Zhang, Z.; Lu, J.; Pei, G. Mitochondria Are Dynamically Transferring Between Human Neural Cells and Alexander Disease-Associated GFAP Mutations Impair the Astrocytic Transfer. Front. Cell. Neurosci. 2019, 13, 316. [Google Scholar] [CrossRef] [Green Version]
  42. D’Souza, A.; Burch, A.; Dave, K.M.; Sreeram, A.; Reynolds, M.J.; Dobbins, D.X.; Kamte, Y.S.; Zhao, W.; Sabatelle, C.; Joy, G.M.; et al. Microvesicles transfer mitochondria and increase mitochondrial function in brain endothelial cells. J. Control. Release 2021, 338, 505–526. [Google Scholar] [CrossRef] [PubMed]
  43. He, K.; Shi, X.; Zhang, X.; Dang, S.; Ma, X.; Liu, F.; Xu, M.; Lv, Z.; Han, D.; Fang, X.; et al. Long-distance intercellular connectivity between cardiomyocytes and cardiofibroblasts mediated by membrane nanotubes. Cardiovasc. Res. 2011, 92, 39–47. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  44. Shen, J.; Zhang, J.; Xiao, H.; Wu, J.; He, K.; Lv, Z.; Li, Z.; Xu, M.; Zhang, Y. Mitochondria are transported along microtubules in membrane nanotubes to rescue distressed cardiomyocytes from apoptosis. Cell Death Dis. 2018, 9, 81. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  45. Ikeda, G.; Santoso, M.R.; Tada, Y.; Li, A.M.; Vaskova, E.; Jung, J.; O’Brien, C.; Egan, E.; Ye, J.; Yang, P.C. Mitochondria-Rich Extracellular Vesicles From Autologous Stem Cell-Derived Cardiomyocytes Restore Energetics of Ischemic Myocardium. J. Am. Coll. Cardiol. 2021, 77, 1073–1088. [Google Scholar] [CrossRef] [PubMed]
  46. Zou, X.; Kwon, S.H.; Jiang, K.; Ferguson, C.M.; Puranik, A.S.; Zhu, X.; Lerman, L.O. Renal scattered tubular-like cells confer protective effects in the stenotic murine kidney mediated by release of extracellular vesicles. Sci. Rep. 2018, 8, 1263. [Google Scholar] [CrossRef] [Green Version]
  47. Gao, J.; Qin, A.; Liu, D.; Ruan, R.; Wang, Q.; Yuan, J.; Cheng, T.S.; Filipovska, A.; Papadimitriou, J.M.; Dai, K.; et al. Endoplasmic reticulum mediates mitochondrial transfer within the osteocyte dendritic network. Sci. Adv. 2019, 5, eaaw7215. [Google Scholar] [CrossRef] [Green Version]
  48. Zampieri, L.X.; Silva-Almeida, C.; Rondeau, J.D.; Sonveaux, P. Mitochondrial Transfer in Cancer: A Comprehensive Review. Int. J. Mol. Sci. 2021, 22, 3245. [Google Scholar] [CrossRef]
  49. Marlein, C.R.; Piddock, R.E.; Mistry, J.J.; Zaitseva, L.; Hellmich, C.; Horton, R.H.; Zhou, Z.; Auger, M.J.; Bowles, K.M.; Rushworth, S.A. CD38-Driven Mitochondrial Trafficking Promotes Bioenergetic Plasticity in Multiple Myeloma. Cancer Res. 2019, 79, 2285–2297. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  50. Dong, L.; Kovarova, J.; Bajzikova, M.; Bezawork-Geleta, A.; Svec, D.; Endaya, B.; Sachaphibulkij, K.; Coelho, A.R.; Sebkova, N.; Ruzickova, A.; et al. Horizontal transfer of whole mitochondria restores tumorigenic potential in mitochondrial DNA-deficient cancer cells. eLife 2017, 6, e22187. [Google Scholar] [CrossRef]
  51. Wang, J.; Liu, X.; Qiu, Y.; Shi, Y.; Cai, J.; Wang, B.; Wei, X.; Ke, Q.; Sui, X.; Wang, Y.; et al. Cell adhesion-mediated mitochondria transfer contributes to mesenchymal stem cell-induced chemoresistance on T cell acute lymphoblastic leukemia cells. J. Hematol. Oncol. 2018, 11, 11. [Google Scholar] [CrossRef]
  52. Burt, R.; Dey, A.; Aref, S.; Aguiar, M.; Akarca, A.; Bailey, K.; Day, W.; Hooper, S.; Kirkwood, A.; Kirschner, K.; et al. Activated stromal cells transfer mitochondria to rescue acute lymphoblastic leukemia cells from oxidative stress. Blood 2019, 134, 1415–1429. [Google Scholar] [CrossRef]
  53. Saha, T.; Dash, C.; Jayabalan, R.; Khiste, S.; Kulkarni, A.; Kurmi, K.; Mondal, J.; Majumder, P.K.; Bardia, A.; Jang, H.L.; et al. Intercellular nanotubes mediate mitochondrial trafficking between cancer and immune cells. Nat. Nanotechnol. 2022, 17, 98–106. [Google Scholar] [CrossRef]
  54. Boudreau, L.H.; Duchez, A.; Cloutier, N.; Soulet, D.; Martin, N.; Bollinger, J.; Paré, A.; Rousseau, M.; Naika, G.S.; Lévesque, T.; et al. Platelets release mitochondria serving as substrate for bactericidal group IIA-secreted phospholipase A2 to promote inflammation. Blood 2014, 124, 2173–2183. [Google Scholar] [CrossRef] [Green Version]
  55. Puhm, F.; Afonyushkin, T.; Resch, U.; Obermayer, G.; Rohde, M.; Penz, T.; Schuster, M.; Wagner, G.; Rendeiro, A.; Melki, I.; et al. Mitochondria Are a Subset of Extracellular Vesicles Released by Activated Monocytes and Induce Type I IFN and TNF Responses in Endothelial Cells. Circ. Res. 2019, 125, 43–52. [Google Scholar] [CrossRef]
  56. Hough, K.P.; Trevor, J.L.; Strenkowski, J.G.; Wang, Y.; Chacko, B.K.; Tousif, S.; Chanda, D.; Steele, C.; Antony, V.B.; Dokland, T.; et al. Exosomal transfer of mitochondria from airway myeloid-derived regulatory cells to T cells. Redox Biol. 2018, 18, 54–64. [Google Scholar] [CrossRef]
  57. Jackson, M.V.; Morrison, T.J.; Doherty, D.F.; McAuley, D.F.; Matthay, M.A.; Kissenpfennig, A.; O’Kane, C.M.; Krasnodembskaya, A.D. Mitochondrial Transfer via Tunneling Nanotubes is an Important Mechanism by Which Mesenchymal Stem Cells Enhance Macrophage Phagocytosis in the In Vitro and In Vivo Models of ARDS. Stem Cells 2016, 34, 2210–2223. [Google Scholar] [CrossRef] [Green Version]
  58. Morrison, T.J.; Jackson, M.V.; Cunningham, E.K.; Kissenpfennig, A.; McAuley, D.F.; O’Kane, C.M.; Krasnodembskaya, A.D. Mesenchymal stromal cells modulate macrophages in clinically relevant lung injury models by extracellular vesicle mitochondrial transfer. Am. J. Respir. Crit. Care Med. 2017, 196, 1275–1286. [Google Scholar] [CrossRef] [Green Version]
  59. Xia, L.; Zhang, C.; Lv, N.; Liang, Z.; Ma, T.; Cheng, H.; Xia, Y.; Shi, L. AdMSC-derived exosomes alleviate acute lung injury via transferring mitochondrial component to improve homeostasis of alveolar macrophages. Theranostics 2022, 12, 2928–2947. [Google Scholar] [CrossRef]
  60. Luz-Crawford, P.; Hernandez, J.; Djouad, F.; Luque-Campos, N.; Caicedo, A.; Carrère-Kremer, S.; Brondello, J.; Vignais, M.; Pène, J.; Jorgensen, C. Mesenchymal stem cell repression of Th17 cells is triggered by mitochondrial transfer. Curr. Stem Cell Res. Ther. 2019, 10, 232. [Google Scholar] [CrossRef]
  61. Court, A.C.; Le-Gatt, A.; Luz-Crawford, P.; Parra, E.; Aliaga-Tobar, V.; Bátiz, L.F.; Contreras, R.A.; Ortúzar, M.I.; Kurte, M.; Elizondo-Vega, R.; et al. Mitochondrial transfer from MSCs to T cells induces Treg differentiation and restricts inflammatory response. EMBO Reports 2020, 21, e48052. [Google Scholar] [CrossRef]
  62. Chen, J.; Wang, Q.; Feng, X.; Zhang, Z.; Geng, L.; Xu, T.; Wang, D.; Sun, L. Umbilical Cord-Derived Mesenchymal Stem Cells Suppress Autophagy of T Cells in Patients with Systemic Lupus Erythematosus via Transfer of Mitochondria. Stem Cells Int. 2016, 2016, 4062789. [Google Scholar] [CrossRef]
  63. Rabas, N.; Palmer, S.; Mitchell, L.; Ismail, S.; Gohlke, A.; Riley, J.S.; Tait, S.W.G.; Gammage, P.; Soares, L.L.; Macpherson, I.R.; et al. PINK1 drives production of mtDNA-containing extracellular vesicles to promote invasiveness. J. Cell Biol. 2021, 220, 1. [Google Scholar] [CrossRef]
  64. Zhang, Z.; Sheng, H.; Liao, L.; Xu, C.; Zhang, A.; Yang, Y.; Zhao, L.; Duan, L.; Chen, H.; Zhang, B. Mesenchymal Stem Cell-Conditioned Medium Improves Mitochondrial Dysfunction and Suppresses Apoptosis in Okadaic Acid-Treated SH-SY5Y Cells by Extracellular Vesicle Mitochondrial Transfer. J. Alzheimer’s Dis. 2020, 78, 1161–1176. [Google Scholar] [CrossRef]
  65. van der Vlist, M.; Raoof, R.; Willemen, H.L.D.M.; Prado, J.; Versteeg, S.; Martin Gil, C.; Vos, M.; Lokhorst, R.E.; Pasterkamp, R.J.; Kojima, T.; et al. Macrophages transfer mitochondria to sensory neurons to resolve inflammatory pain. Neuron 2022, 110, 613–626.e9. [Google Scholar] [CrossRef]
  66. Peruzzotti-Jametti, L.; Bernstock, J.D.; Willis, C.M.; Manferrari, G.; Rogall, R.; Fernandez-Vizarra, E.; Williamson, J.C.; Braga, A.; van den Bosch, A.; Leonardi, T.; et al. Neural stem cells traffic functional mitochondria via extracellular vesicles. PLoS Biol. 2021, 19, e3001166. [Google Scholar] [CrossRef]
  67. Levoux, J.; Prola, A.; Lafuste, P.; Gervais, M.; Chevallier, N.; Koumaiha, Z.; Kefi, K.; Braud, L.; Schmitt, A.; Yacia, A.; et al. Platelets facilitate the wound-healing capability of mesenchymal stem cells by mitochondrial transfer and metabolic reprogramming. Cell Metab. 2021, 33, 688–690. [Google Scholar] [CrossRef]
  68. Ahmad, T.; Mukherjee, S.; Pattnaik, B.; Kumar, M.; Singh, S.; Kumar, M.; Rehman, R.; Tiwari, B.K.; Jha, K.A.; Barhanpurkar, A.P.; et al. Miro1 regulates intercellular mitochondrial transport & enhances mesenchymal stem cell rescue efficacy. EMBO J. 2014, 33, 994–1010. [Google Scholar] [CrossRef]
  69. Zhang, Y.; Yu, Z.; Jiang, D.; Liang, X.; Liao, S.; Zhang, Z.; Yue, W.; Li, X.; Chiu, S.; Chai, Y.; et al. iPSC-MSCs with High Intrinsic MIRO1 and Sensitivity to TNF-α Yield Efficacious Mitochondrial Transfer to Rescue Anthracycline-Induced Cardiomyopathy. Stem Cell Rep. 2016, 7, 749–763. [Google Scholar] [CrossRef] [Green Version]
  70. Rustom, A.; Saffrich, R.; Markovic, I.; Walther, P.; Gerdes, H. Nanotubular Highways for Intercellular Organelle Transport. Science 2004, 303, 1007–1010. [Google Scholar] [CrossRef]
  71. Wang, Y.; Cui, J.; Sun, X.; Zhang, Y. Tunneling-nanotube development in astrocytes depends on p53 activation. Cell Death Differ. 2011, 18, 732–742. [Google Scholar] [CrossRef] [Green Version]
  72. Takatsu, H.; Kawano, S.; Watarai, H.; Kimura, S.; Yeaman, C.; Ohno, H.; Ohmae, M.; Kitamura, H.; Hase, K.; Hazelett, C.C.; et al. M-Sec promotes membrane nanotube formation by interacting with Ral and the exocyst complex. Nat. Cell Biol. 2009, 11, 1427–1432. [Google Scholar] [CrossRef]
  73. Wang, Y.; Ni, J.; Gao, T.; Gao, C.; Guo, L.; Yin, X. Activation of astrocytic sigma-1 receptor exerts antidepressant-like effect via facilitating CD38-driven mitochondria transfer. Glia 2020, 68, 2415–2426. [Google Scholar] [CrossRef]
  74. Sun, X.; Wang, Y.; Zhang, J.; Tu, J.; Wang, X.; Su, X.; Wang, L.; Zhang, Y. Tunneling-nanotube direction determination in neurons and astrocytes. Cell Death Dis. 2012, 3, e438. [Google Scholar] [CrossRef] [Green Version]
  75. MacAskill, A.F.; Rinholm, J.E.; Twelvetrees, A.E.; Arancibia-Carcamo, I.L.; Muir, J.; Fransson, A.; Aspenstrom, P.; Attwell, D.; Kittler, J.T. Miro1 Is a Calcium Sensor for Glutamate Receptor-Dependent Localization of Mitochondria at Synapses. Neuron 2009, 61, 541–555. [Google Scholar] [CrossRef] [Green Version]
  76. Misko, A.; Jiang, S.; Wegorzewska, I.; Milbrandt, J.; Baloh, R.H. Mitofusin 2 Is Necessary for Transport of Axonal Mitochondria and Interacts with the Miro/Milton Complex. J. Neurosci. 2010, 30, 4232–4240. [Google Scholar] [CrossRef] [Green Version]
  77. van Niel, G.; D’Angelo, G.; Raposo, G. Shedding light on the cell biology of extracellular vesicles. Nat. Rev. Mol. Cell Biol. 2018, 19, 213–228. [Google Scholar] [CrossRef]
  78. Todkar, K.; Chikhi, L.; Desjardins, V.; El-Mortada, F.; Pépin, G.; Germain, M. Selective packaging of mitochondrial proteins into extracellular vesicles prevents the release of mitochondrial DAMPs. Nat. Commun. 2021, 12, 1971. [Google Scholar] [CrossRef]
  79. Sugiura, A.; McLelland, G.; Fon, E.A.; McBride, H.M. A new pathway for mitochondrial quality control: Mitochondrial-derived vesicles. EMBO J. 2014, 33, 2142–2156. [Google Scholar] [CrossRef] [Green Version]
  80. Tan, Y.L.; Eng, S.P.; Hafez, P.; Abdul Karim, N.; Law, J.X.; Ng, M.H. Mesenchymal Stromal Cell Mitochondrial Transfer as a Cell Rescue Strategy in Regenerative Medicine: A Review of Evidence in Preclinical Models. Stem Cells Transl. Med. 2022, 11, 814. [Google Scholar] [CrossRef]
Biomolecules 12 01770 g001 550
Figure 1. Schematic representations of mitochondrial disposal processes. (A) Exopher-mediated mitochondrial disposal process. (B) Mitocytosis, a migrasome-mediated mitochondrial disposal process. See text for details and definitions of abbreviations. Drp1: dynamin-related protein 1, KIF5B: kinesin family member 5B, Myo19: myosin XIX.
Figure 1. Schematic representations of mitochondrial disposal processes. (A) Exopher-mediated mitochondrial disposal process. (B) Mitocytosis, a migrasome-mediated mitochondrial disposal process. See text for details and definitions of abbreviations. Drp1: dynamin-related protein 1, KIF5B: kinesin family member 5B, Myo19: myosin XIX.
Biomolecules 12 01770 g001
Biomolecules 12 01770 g002 550
Figure 2. Schematic representations of mechanisms underlying mitochondrial release or transfer from cells. (A) Tunneling nanotube (TNT)-mediated intercellular transfer of mitochondria. (B) Extracellular vesicle (EV)-mediated mitochondrial release/transfer from cells. See text for details and definitions of abbreviations. CD38: cluster of differentiation 38, Cdc42: Cell division control protein 42, ERK1/2: extracellular regulated protein kinases 1/2, MDV: mitochondrial-derived vesicle, OPA1: Optic atrophy 1, PRKN: Parkin, RalA: Ras-related protein A. S100A4: S100 calcium binding protein A4, Snx9: Sorting nexin-9.
Figure 2. Schematic representations of mechanisms underlying mitochondrial release or transfer from cells. (A) Tunneling nanotube (TNT)-mediated intercellular transfer of mitochondria. (B) Extracellular vesicle (EV)-mediated mitochondrial release/transfer from cells. See text for details and definitions of abbreviations. CD38: cluster of differentiation 38, Cdc42: Cell division control protein 42, ERK1/2: extracellular regulated protein kinases 1/2, MDV: mitochondrial-derived vesicle, OPA1: Optic atrophy 1, PRKN: Parkin, RalA: Ras-related protein A. S100A4: S100 calcium binding protein A4, Snx9: Sorting nexin-9.
Biomolecules 12 01770 g002
Biomolecules 12 01770 g003 550
Figure 3. Schematic hypothetical model of the mitochondrial quality control system in cardiomyocytes. Under physiological conditions, both the intracellular mitochondrial quality control systems, such as mitophagy, and extracellular mitochondrial ejection equivalently contribute to the removal of damaged mitochondria. However, the demand for extracellular clearance of damaged mitochondria is markedly increased under stress conditions in cardiomyocytes. Explanation red arrow: increasing.
Figure 3. Schematic hypothetical model of the mitochondrial quality control system in cardiomyocytes. Under physiological conditions, both the intracellular mitochondrial quality control systems, such as mitophagy, and extracellular mitochondrial ejection equivalently contribute to the removal of damaged mitochondria. However, the demand for extracellular clearance of damaged mitochondria is markedly increased under stress conditions in cardiomyocytes. Explanation red arrow: increasing.
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Table
Table 1. Summary of the reports regarding mitochondrial release and/or transfer from various cells.
Table 1. Summary of the reports regarding mitochondrial release and/or transfer from various cells.
DonorAcceptorStimulationComponentsOutcomeRoutesRef.
AdipocytesCardiomyocytesMitochondrial stressDamaged mitochondriaBurst of ROS; protect the heart through hormesisEVs[24]
hMSCsA549 cell line (NSCLC-derived) Mitochondria and mtDNARescued aerobic respiration [27]
MSCsCardiomyoblastsIschemiaMitochondriaReduced cell death [28]
BMMSCsH9c2 cell lineIschemia/reperfusionMitochondriaReduced apoptosisTNTs[29]
MSCsCardiomyocytes Mitochondria [30]
MSCsICMsDoxorubicin administrationMitochondriaImproved ICM contractility and mitochondrial biogenesis EVs[31]
BMSCsAlveolar epitheliaAcute lung injury (ALI) caused by lipopolysaccharide (LPS)MitochondriaReduced acute lung injury,
increased alveolar ATP concentrations		Gap junctions and MVs[32]
iPSC-MSCs Epithelial cells MitochondriaImproved mitochondrial function, reduced inflammationTNTs[33]
iPSC-MSCsEpithelial cellsCigarette smokeMitochondriaAlleviates alveolar fibrosisTNTs[34]
MMSCsNeuronal cells MitochondriaAlleviated stroke-induced damage [35]
MSCsMouse neuronsHydrogen peroxide exposureMitochondriaIncreased neuronal survival and improved metabolism [36]
MMSCsNeuronsOxygen-glucose deprivationMitochondriaRestored Cell Proliferation and respirationTNTs [37]
MSCsNeural stem cellsCo-culture with cisplatin damaged NSCsMitochondriaNormalized mitochondrial membrane potential, prevented cell deathTNTs[38]
AstrocytesNeuronsIschemiaFunctional mitochondriaIncreased neuronal viability and ATP levelsMVs[39]
Astrocytes NeuronsCisplatin treatmentMitochondriaIncreased neuronal survival, restored neuronal mitochondrial membrane potential, and normalized neuronal calcium dynamics [40]
Astrocytes or neuronal cellsAstrocytes MitochondriaElevated mitochondrial membrane potential [41]
hCMEC/D3
(human brain EC cell line)		Brain ECs and neuronsIschemiaPolarized mitochondriaIncreased ATP levelsEVs[42]
CardiomyocytesCardiofibroblasts Mitochondria TNTs[43]
Cardiac myofibroblastsCardiomyocytesHypoxia/reoxygenationMitochondriaReduced apoptosisTNTs[44]
Human-iPS cell-derived cardiomyocytes (iCMs)Cardiomyocytes MitochondriaRestoration of bioenergetics and mitochondrial biogenesisEVs[45]
Renal scattered tubular cellsTubular epithelial cells MitochondriaImproved mitochondrial function (in vitro), perfusion and oxygenation(in vivo)EVs[46]
B16ρ0 mouse melanoma cells MitochondriaRescued mitochondrial function [50]
BMSCsMultiple myeloma cells MitochondriaIncreased ATP levels and proliferation TNTs[49]
MSCsJurkat cellsChemotherapeutic drugsMitochondriaChemoresistanceTNTs[51]
MSCsPrimary bone marrow cells of ALL patients Chemotherapeutic drugsMitochondriaReduced apoptosisTNTs[52]
NKT cells (DN32.D3, mouse T cells)Cancer cells (MDA-MB-231, 4T1, TALL-104) MitochondriaEnhanced cancer cell activity and caused death of immune cells TNTs[53]
MDA-MB-231 breast cancer cellsMDA-MB-231 breast cancer cellsActivation of mGluR3 by extracellular glutamatemtDNAPromote endosomal trafficking and invasiveness MVs[63]
Human umbilical cord derived MSC-CMSH-SY5Y cellsOA(okadaic acid) treatmentMitochondria Alleviated oxidative stress, suppressed apoptosis, improved mitochondrial functionMVs[64]
MSCsMacrophageAcute respiratory distress syndrome (ARDS)MitochondriaPromote an anti-inflammatory and highly phagocytic macrophage phenotypeMVs[58]
MacrophagesSensory neuronsInflammationMitochondriaResolution of inflammatory painEVs[65]
Airway myeloid-derived regulatorycellsT cells Polarized mitochondria and mtDNA EVs[56]
Neural stem cellmtDNA-deficient L929 Rho0 cells
(mononuclear phagocytes)		 Functional mitochondriaRescued mitochondrial function, increased cell survival, reduced the expression of pro-inflammatory markersEVs[66]
PlateletsMSC MitochondriaImproved the regenerative capacityEVs[67]
MSCsEpithelial cellStress induction by rotenone or TNF-αMitochondriaReduced ROS productionTNTs[68]
MSCscardiomyocytesAnthracycline or DoxMitochondriaRescued damageTNTs[69]
NSCLC: Non-small cell lung cancer, EC: endothelial cell, iPSC: induced pluripotent stem cell, BMSC: Bone marrow stromal cells, EV: extracellular vesicles, TNT: tunneling nanotubes.
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Fan, Q.; Maejima, Y.; Wei, L.; Nakagama, S.; Shiheido-Watanabe, Y.; Sasano, T. The Pathophysiological Significance of “Mitochondrial Ejection” from Cells. Biomolecules 2022, 12, 1770. https://doi.org/10.3390/biom12121770

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Fan Q, Maejima Y, Wei L, Nakagama S, Shiheido-Watanabe Y, Sasano T. The Pathophysiological Significance of “Mitochondrial Ejection” from Cells. Biomolecules. 2022; 12(12):1770. https://doi.org/10.3390/biom12121770

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Fan, Qintao, Yasuhiro Maejima, Lai Wei, Shun Nakagama, Yuka Shiheido-Watanabe, and Tetsuo Sasano. 2022. "The Pathophysiological Significance of “Mitochondrial Ejection” from Cells" Biomolecules 12, no. 12: 1770. https://doi.org/10.3390/biom12121770

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