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Review

The role of Mitochondrial Fission Proteins in Mitochondrial Dynamics in Kidney Disease

by
Lingyu Qin
and
Shuhua Xi
*
Department of Environmental Health, School of Public Health, China Medical University, No. 77 Puhe Road, Shenyang North New Area, Shenyang 110122, China
*
Author to whom correspondence should be addressed.
Int. J. Mol. Sci. 2022, 23(23), 14725; https://doi.org/10.3390/ijms232314725
Submission received: 29 September 2022 / Revised: 27 October 2022 / Accepted: 2 November 2022 / Published: 25 November 2022
(This article belongs to the Section Molecular Pathology, Diagnostics, and Therapeutics)
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Abstract

:
Mitochondria have many forms and can change their shape through fusion and fission of the outer and inner membranes, called “mitochondrial dynamics”. Mitochondrial outer membrane proteins, such as mitochondrial fission protein 1 (FIS1), mitochondrial fission factor (MFF), mitochondrial 98 dynamics proteins of 49 kDa (MiD49), and mitochondrial dynamics proteins of 51 kDa (MiD51), can aggregate at the outer mitochondrial membrane and thus attract Dynamin-related protein 1 (DRP1) from the cytoplasm to the outer mitochondrial membrane, where DRP1 can perform a scissor-like function to cut a complete mitochondrion into two separate mitochondria. Other organelles can promote mitochondrial fission alongside mitochondria. FIS1 plays an important role in mitochondrial–lysosomal contacts, differentiating itself from other mitochondrial-fission-associated proteins. The contact between the two can also induce asymmetric mitochondrial fission. The kidney is a mitochondria-rich organ, requiring large amounts of mitochondria to produce energy for blood circulation and waste elimination. Pathological increases in mitochondrial fission can lead to kidney damage that can be ameliorated by suppressing their excessive fission. This article reviews the current knowledge on the key role of mitochondrial-fission-associated proteins in the pathogenesis of kidney injury and the role of their various post-translational modifications in activation or degradation of fission-associated proteins and targeted drug therapy.

1. Introduction

Mitochondria are the main site of respiration, producing ATP through oxidative phosphorylation (OXPHOS) to supply cells and organisms with vital activities [1]. Additionally, mitochondria have demonstrated excellent immunological effects against bacterial infections and viral infections. In past decades, research has been focused on mitochondrial bioenergetics, but, in recent years, the complexity and versatility of mitochondrial activities have been realized [2]. Individual mitochondria exist in various forms, such as small spherical, shorter, and longer tubular forms. However, further studies reveal that their different morphologies can be inter-connected and that the mitochondrial network can be regulated by the binding and breaking of the outer and inner mitochondrial membranes, a process called “mitochondrial dynamics” [3]. Mitochondrial fission and fusion mechanisms produce new mitochondria while eliminating old, damaged, and irreparable ones [4]. Mitochondrial fission proteins FIS1 and DRP1 are also involved in the cell cycle and cytoskeleton, thereby triggering fission. In contrast, the mitochondrial fusion proteins MFN1/MFN2 also play an important role in cell proliferation. Promoting mitochondrial-fission-related protein expression increases mitochondrial network fragmentation, while increasing mitochondrial fission promotes cytochrome C release from mitochondria and thus increases apoptosis, while inhibiting mitochondrial-fission-related proteins reduces mitochondrial fission and inhibits apoptosis to promote cell survival [5,6].
The kidney is the second most energy-demanding organ in the body after the heart [7]. The kidney has a large energy demand, and it needs much energy to finish cleaning the metabolic waste from the body’s blood. Hence, its mitochondrial content ranks high among many organs. When kidneys develop a disease, the mitochondria also appear abnormal. The mitochondria appear fragmented in kidney cells of patients with diabetic nephropathy, and the mitochondrial dynamics associated with protein DRP1 are often in an activated state of phosphorylation, leading to an increase in mitochondrial fission [8]. However, when mitochondrial fission increases, the permeability of the outer mitochondrial membrane increases, resulting in the release of its contents and a decrease in mitochondrial function, which can cause kidney cell damage, and inhibiting the increase in mitochondrial fission can protect kidney cells [9,10].

2. Mitochondrial Dynamics

Mitochondria are powerful organelles, and the mitochondrial network plays an important function in the cell by providing energy, regulating programmed cell death, and producing reactive oxygen species (ROS) [11]. Mitochondria are composed of the outer mitochondrial membrane (OMM), inner mitochondrial membrane (IMM), cristae, matrix, and intermembrane space (IMS) (Figure 1). The OMM separates the mitochondria from the cell matrix, while the IMM forms cristae and can separate the mitochondrial matrix from the outer membrane interstitial region. In the past, mitochondria were often thought to exist in isolation, but they form highly dynamic mitochondrial networks interacting with each other. Furthermore, mitochondrial networks are not static, and the interaction between OMM and IMM of different mitochondria can change the mitochondrial network morphology [12,13]. While “mitochondrial dynamics” consists primarily of fission and fusion, many researchers include cristae remodeling in this category. It has been demonstrated that mitochondrial fission is commonly associated with mitochondrial dysfunction, whereas mitochondrial fusion can serve a protective function [14]. In cellular life activities, mitochondrial fusion and fission can occur in a short period, especially in the case of external-stress-induced fission or transient partial fusion events [15]. Fusion and fission are “double-edged swords” that are important for normal mitochondrial function. Mitochondrial fission produces small spherical mitochondria that play an important role in axonal cell transport, while mitochondrial fusion protects against external stimuli [16]. A decrease or increase in mitochondrial fission and fusion can lead to imbalances that affect mitochondrial function and ultimately lead to various diseases [17]. Normal cristae play an important role in cell metabolism and cell death, and reducing the width of cristae enhances ATP production and resistance to external death stimuli [18,19].

2.1. Mitochondrial Fission

Mitochondrial fission is the splitting of an intact mitochondrion into two separate mitochondria. Multiple factors, including the endoplasmic reticulum, lysosomes, Golgi-derived vesicles, and actin filaments, regulate mitochondrial fission [20,21,22,23,24]. Mitochondrial fission begins with labeling fission sites, usually the contact sites of the nucleoid markers of the mitochondrial matrix, the endoplasmic reticulum, and lysosomes [25,26]. Next, mitochondrial outer membrane protein proteins, including FIS1, MFF, MiD49, and MiD51, aggregate at a site in the mitochondrial outer membrane. The mitochondrial outer membrane protein receptor recruits the DRP1 from the cytoplasm to the site of mitochondrial fission (Figure 2). DRP1, a cytosolic dynamin GTPase, plays an important role in mitochondrial fission [27]. DRP1 can form oligomeric rings, and, as DRP1 aggregation increases, a hinge-like structure can form, severing OMM and IMM simultaneously [28]. FIS1 can reduce the number and viability of mitochondrial fusion proteins (MFN1, MFN2, and OPA1) by binding to them and fragmenting the mitochondrial network [29,30]. While it was thought that the inner and outer membranes were fissioned simultaneously during mitochondrial fission, new insights suggest that inner mitochondrial membrane fission is independent and increased short OPA1 isoform (S-OPA1) accumulation and translocated IMM protein mitochondrial protein 18 kDa (MTP18) expression can mediate IMM fission [28,31]. However, this latter view needs to be further tested.

2.2. Mitochondrial Fusion

Mitochondrial fusion refers to fusion of several mitochondria with intact structures into one longer mitochondrion. Mitochondrial fusion is divided into two parts, outer mitochondrial membrane fusion and inner membrane fusion. In the past, it was thought that the outer and inner mitochondrial membranes fused nearly simultaneously [32]. However, recent literature reports that IMM and OMM fusions are continuous, and mitochondrial fusion can be divided into “transient fusions” and “complete fusions”. Transient fusions typically interact obliquely or horizontally and, to a lesser extent, vertically; however, transient fusions tend to preserve the original mitochondrial morphology, whereas complete fusions are frequently longitudinal and capable of producing a complete mitochondrion [33]. MFN1 and MFN2 mediate outer membrane fusion in mammals (Figure 2) [34]. MFN1 and MFN2 proteins can interact between mitochondria, tethering two separate mitochondrial outer membranes via their HR2 structural domains [35,36]. This is the beginning of fission [37]. Moreover, MFN2 can act as a physical tether between mitochondria and the endoplasmic reticulum and regulate calcium ion signaling [38]. However, recent studies suggest that MFN2 has the opposite effect [39]. The specific role of MFN2 needs to be studied specifically in the context of different mechanisms of action in various cells. OPA1 plays an important role in IMM fusion [40]. OMA1 and AAA protease YME1L, mitochondrial proteases, can cleave OPA1 from the long (L-OPA1) to the short (S-OPA1) form. L-OPA1 is needed for mitochondrial fusion, while S-OPA1 is needed for mitochondrial fission [41]. OPA1 downregulation inhibits mitochondrial fusion, resulting in mitochondrial fragmentation [42]. Its upregulation can promote the fusion of mitochondria to protect cells via an anti-apoptotic effect. The use of drugs to increase OPA1 expression is of great research value for cytoprotection [43]. OPA1 can inhibit apoptosis independently of mitochondrial fusion and reduce cytochrome C release [44].

2.3. Cristae Remodeling

Cristae remodeling refers to changes in the length, width, abundance, and exit of the cristae in response to external stimuli [28]. Cristae morphology is related to the efficiency of energy production, apoptosis, and oxidative stress [45]. L-OPA1 and S-OPA1 can form oligomers that act as “gatekeepers” under normal conditions (Figure 3). When the cristae opening becomes larger and L-OPA1 decreases, cytochrome C that remains in the cristae is released, triggering a series of cell death behaviors [44].

2.4. Mitochondrial Dynamics with Other Cellular Organelles

2.4.1. Endoplasmic Reticulum

The mitochondria and endoplasmic reticulum (ER) can interact through protein–protein interactions, and the distance between them can be decreased to form contact sites (Figure 4). ER and mitochondria interaction is critical for calcium homeostasis and mitochondrial dynamics. At the ER–mitochondrial contact site, mitochondrial contraction followed by mitochondrial division has been observed [20]. ER tubules wrapped around the mitochondria can mark the site of DRP1 recruitment by the mitochondrial receptor; the assembled DRP1 aggregates and then forms a helix to contract the mitochondria; ER tubules play a localization role in mitochondrial division and even participate in mitochondrial fission. DRP1 cooperates with formin 2 (INF2) on the ER and the formin-binding protein spire 1C on the outer mitochondrial membrane, leading to actin accumulation before DRP1 recruitment to the fission site, thereby promoting mitochondrial precontraction [23]. The connection between the ER and the mitochondrial membrane results from the protein complex’s physical binding. The first is a complex between FIS1 on the mitochondrial membrane and BAP31 on the ER, frequently associated with cell death, and the second is that MFN2 also plays an important role in the contact between the two [46]. ER structures, particularly renal tubule ER–mitochondrial contacts, are necessary for steady-state mtDNA replication, and mtDNA-containing nucleoids are early markers of nascent mitochondrial division sites [47]. According to the literature, ORP1L-mediated PI(4)P signaling at the ER–lysosomal–mitochondrial three-way contact contributes to mitochondrial division [48].

2.4.2. Lysosomes

Mitochondrial–lysosomal contacts are also critical and play an important role in several diseases. Various protein mechanisms on the mitochondrial and lysosomal membranes regulate mitochondrion–lysosome contact site tethering. It can function as a linkage through the binding of the RAB7GTP protein on the lysosomal surface and an unknown mitochondrial protein (Figure 4) [49]. FIS1 is a mitochondrial-fission-related outer mitochondrial membrane protein that recruits TBC1D15, the activator protein of RAB7GTP, to the mitochondria and induces RAB7GTP conversion on lysosomes to RAB7GDP, thereby unbinding the mitochondria from the lysosomes [21]. Lysosomal dissociation from the mitochondrial division site increases mitochondrial fission [49].

2.4.3. Golgi

Mitochondrial dynamics are related to numerous organelles, and mitochondrial division is related to the ER, lysosomes, and Golgi. Arf proteins are small GTP-binding (G) proteins. Arf proteins are classified into three groups; Arf1 is highly conserved in evolutionary time and plays an important role in the structure and function of the Golgi [50]. Arf1 and PI(4)KIIIβ are mainly restricted to the Golgi apparatus, and Arf1 can activate PI(4)KIIIβ to produce PI(4)P, which is involved in late mitochondrial fission (Figure 4) [51].

2.4.4. Actin

It has been demonstrated that mitochondrial fission requires preconstruction, which is inseparable from the actin cytoskeleton, and that the proteins involved, Spire1C and INF2, play an important role in inducing mitochondrial constriction (Figure 4) [52]. Spire1C is a protein on the OMM, and the ER-anchored junctional isoform of INF2 can promote mitochondrial constriction by regulating its actin polymerization activity. Spire1C interacts with INF2 to drive actin filament formation in narrowed mitochondria [24]. It can further promote the contact between mitochondria and ER and mitochondrial fission.

2.5. ROS in Mitochondrial Dynamics

ROS are small, highly reactive molecules that oxidize proteins, lipids, and DNA [53]. In mammals, mitochondria are the primary source of ROS. Additionally, ROS can promote mitochondrial fission by increasing mitochondrial fission proteins and inducing post-translational modifications to promote apoptosis [54,55,56]. Persistent mitochondrial fragmentation in cells has been observed to be frequently associated with elevated ROS [57,58]. ROS plays an important potential role in promoting mitochondrial fission. When external stimuli, such as hypoxia or drug interventions, cause elevated intracellular ROS, they frequently cause an increase in mitochondrial-fission-related proteins DRP1 and FIS1 and promote their post-translational modification to activate fission-related proteins, resulting in a pathological increase in mitochondrial fission that can have adverse effects on cells [59,60].

3. Structure and Function of Mitochondrial Fission Proteins FIS1/DRP1 and the Role of Post-Translational Modifications

Mitochondrial fission is not only ordinary monotonic fission; mitochondrial fission is divided into midzone and peripheral fission. Peripheral fission upstream displays signs of stress and damage that may lead to degradation, while midzone fission may contribute to biogenesis. Peripheral fission is inseparable from the role of FIS1 [61]. FIS1 deletion prevents apoptosis upstream of Bax translocation, whereas DRP1 deletion protects cells downstream of Bax translocation and upstream of cytochrome C release [32,62]. BAK and BAX can oligomerize on the OMM to drive its rupture. Subsequent increases in mitochondrial outer membrane permeability (MOMP) lead to outflow of pro-apoptotic factors (including cytochrome C and mtDNA) into the cytoplasmic matrix, triggering various programmed cell deaths. In addition to causing mitochondrial fission, FIS1/DRP1 interaction has been demonstrated to cause mitochondrial dysfunction in cells, such as decreased mitochondrial membrane potential, oxidative stress, and bioenergetic failure. When inhibitors that inhibit the interaction between the two are used, mitochondrial dysfunction can be effectively improved [63]. This indicates that DRP1 and FIS1 play a significant role in mitochondrial dynamics and apoptosis. Protein post-translational modifications (PTMs) occur when enzymes catalyze one or more amino acid residues of a protein to increase or decrease a chemical group, resulting in the protein’s degradation or activation. Popularly speaking, post-translation modification refers to chemical modification of proteins after translation. Only the structures of the mitochondrial fission proteins FIS1 and DRP1 and the role played by post-translational modifications in the regulation of protein function are highlighted here.

3.1. FIS1

3.1.1. Structure and Function of FIS1

FIS1 has a flexible N-terminal tail, six a-helices connected by short loops to form a core domain structurally similar to a tridecapeptide repeat (TPR), and a disordered C-terminus containing a transmembrane region (TMD) (Figure 5) [64,65]. According to studies, the N-terminal structure of FIS1 is important for its mitochondrial fission activity [66]. The TPR-like structural domain is a helix-rotation helix pattern that is usually organized into a tandem structure capable of mediating protein–protein interactions that are critical to its biological function [67]. While the TMD plays a role in transporting the protein to the outer mitochondrial membrane, without this region, FIS1 would not be able to localize to the mitochondria and diffuse in the cytoplasmic region [64].
FIS1 can recruit DRP1 to the OMM to promote mitochondrial fission [63,68,69,70,71,72]. However, recent research discovered that mitochondria could regulate contact with lysosomes through FIS1 to trigger asymmetric mitochondrial division [61,73]. FIS1 overexpression can lead to mitochondrial fragmentation during acute kidney injury [74]. The same can happen in children with membranous nephropathy [75]. High expression of FIS1 promotes mitochondrial division, apoptosis, and pyroptosis of cells, thus inducing nephrotoxicity [76]. However, it has also been shown that FIS1 also plays an important role in mitochondrial autophagy and can play a protective role in diabetic nephropathy by participating in mitochondrial quality control through the adaptive mitochondrial autophagy pathway [77].

3.1.2. Post-Translational Modifications of FIS1 during Mitochondrial Fission

FIS1 is mainly regulated by several post-translational modifications, mainly including: phosphorylation, ubiquitination, SUMOylation, and acetylation (Table 1). These modifications play an important role in activation and degradation of FIS1.

Phosphorylation

Phosphorylation is widespread post-translational modification of proteins and plays an important role in regulating protein and cellular functions. Although numerous phosphorylation sites have been identified, this is only the tip of the iceberg; more sites remain to be discovered [78]. Phosphorylation is most common at serine, followed by threonine and tyrosine, which occur at a frequency of approximately 11.2:2.5:1 but can also occur at other additional sites [79]. FIS1 can be directly phosphorylated at the tyrosine 38 site (Tyr38) by other factors, such as MET, and FIS1 pY38 can recruit Drp1 to promote mitochondrial fission, resulting in fragmented mitochondrial networks [68]. Studies have demonstrated that DNA-dependent protein kinase catalytic subunit (DNA-PKcs) can phosphorylate Fis1 [80]. Phosphorylation on FIS1 promotes mitochondrial fission. In the case of increased pathological mitochondrial fission due to kidney injury, phosphorylation of FIS1 can be inhibited to play a role in mitigating injury and protection, introducing a new idea of therapeutic protection.

Ubiquitination

Ubiquitin (Ub) is a relatively conserved protein that is often associated with protein degradation [81]. Ubiquitin is a 76-amino-acid protein and, therefore, has many potential sites for additional post-translational modifications [82]. Ubiquitination covalently couples to lysine residues on target proteins through a series of enzymatic reactions that activate (E1), conjugate (E2), and ligate (E3) enzymes. Parkin is an E3 ubiquitin ligase that regulates ubiquitination of its substrates and can mediate protein degradation [83]. PINK can regulate Parkin activity by regulating Parkin phosphorylation, so PINK/Parkin is often used in combination to regulate protein activity in mitochondria [84,85]. FIS1 is one of the targets of Parkin-mediated ubiquitination and is able to degrade FIS1 [86]. It has also been shown that MARCH5/MITOL (E3 ligase) can influence mitochondrial morphology by affecting FIS1 [87,88].

SUMOylation

Sentrin/small-ubiquitin-related modifier (SUMO) can regulate protein modification pathways for a variety of biological processes, such as cell division, DNA replication and repair, cell death, and cellular metabolism. SUMOylation works somewhat similar to ubiquitination, which is why SUMOization is also called mini-ubiquitination. However, the enzymes involved in the two are completely different. Another difference between the two is that ubiquitination is relatively complex, while the biochemical reactions of SUMOization and de-SUMOization are relatively mild [89]. SUMO couples to lysine residues in target proteins via SUMO-specific activating (E1), conjugating (E2), and ligating (E3) enzyme-catalyzed isopeptide bonds. SUMOylation is a reversible process and can be de-SUMOylated by the activity of the SENP protease family [90]. The lysine 149 site (K149) of FIS1 can be SUMOized. Blocking SUMOylation of Fis1 enhances Fis1 mitochondrial localization [91]. SENP3, a member of the SENP protease family, is a de-SUMOized enzyme that de-SUMO-izes FIS1, thereby enhancing its mitochondrial targeting.

Acetylation

Lysine acetylation (acetylation) is a reversible post-translational modification that plays an essential role as a player in the life processes of many cells. Acetylation is mainly regulated by lysine acetyltransferases (KATs) and lysine deacetylases (HDAC). Acetylation is widespread, and the acetylation status of many sites is controlled by the enzymatic activity of NAD-dependent deacetylase Sirtuin 3 (SIRT3). SIRT3 is the only mitochondrial member with strong deacetylation activity; SIRT3 is the major NAD-dependent lysine deacetylase in mitochondria, with many acetylation sites in mitochondrial proteins that are involved in mitochondrial dynamics, ATP production, pyruvate metabolism, and antioxidant defense [92,93,94]. SIRT3 plays an important role in mitochondrial fission, and knockdown of SIRT3 increases FIS1 expression and increases mitochondrial fragmentation [95,96]. SIRT3 is essential for maintaining the balance between mitochondrial fission and fusion.

3.2. DRP1

3.2.1. Structure and Function of DRP1

DRP1 is a cytoplasmic guanosine triphosphatase that is activated and can be recruited from the cytoplasm to the OMM by mitochondrial outer membrane proteins. DRP1 protein is known to have four structural domains: the C-terminal GTPase effector domain (GED), the variable structural domain (variable), the helical intermediate structural domain (middle), and the highly conserved N-terminal GTPase structural domain (GTPase) (Figure 6). The DRP1 protein is recruited to the membrane by the receptor protein on the OMM and then severs the inner and outer mitochondrial membranes by forming a dimer or tetramer through a variable structural domain and binding to the outer mitochondrial membrane to act as a hinge [97].
DRP1 promotes mitochondrial fission, increased expression of DRP1 promotes fragmentation of the mitochondrial network, while inhibition of DRP1 expression can lead to highly elongated mitochondria [98]. In diabetic nephropathy, mitochondrial fission can be reduced by decreasing DRP1 expression to stop progression of diabetic nephropathy [99]. Inhibition of DRP1 plays an important protective role in protection against ischemic acute kidney injury [100].

3.2.2. Post-Translational Modifications of DRP1 during Mitochondrial Fission

DRP1 is mainly regulated by the following post-translational modifications: phosphorylation, ubiquitination, SUMOylation, O-GlcNAcylation, acetylation, S-Nitrosylation, etc (Table 2). These modifications mainly occur in the variable structural domain and the C-terminal GTPase effector structural domain.

Phosphorylation

There are usually many phosphorylation sites of DRP1, such as serine sites: Ser-40, Ser-44, Ser-579, Ser-585, Ser-592, Ser-616, Ser-637, Ser-656, and Ser-693 [101]. The most studied DRP1 phosphorylation sites are Ser-616 and Ser-637. Activation of the Ser-616 site of DRP1 promotes DRP1 movement from the cytoplasm to the OMM, interacting with OMM proteins and thus promoting mitochondrial fission [102]. There are many proteins that can activate the Ser-616 site of DRP1, such as Stat2, Rho-associated protein kinase (ROCK), PKCδ, ERK1/2, calmodulin-dependent protein kinase II (CaMKII), and Cdk5 [103,104,105,106,107,108,109]. In contrast, the Ser-637 and Ser-616 sites of DRP1 have opposite effects. Ser-637 plays an inhibitory role on DRP1, and inactivation of DRP1 inhibits DRP1 translocation to the OMM, thus reducing mitochondrial fission [110,111]. The Ser-637 site of DRP1 is normally regulated by, PKA, PKD, CaN, and AMPK [112].

Ubiquitination

Inactivation of Parkin often leads to reduced degradation of Drp1, resulting in increased translocation of Drp1 activity, leading to excessive mitochondrial division and ultimately to development of certain diseases [101]. MRCH5 is an OMM-related E3 ubiquitin ligase that controls mitochondrial function [113]. According to the literature, MARCH5 plays a crucial role in controlling mitochondrial morphology by regulating Drp1 activity [114]. Some studies have demonstrated that SQSTM1/P62 has the same effect on DRP1 [115,116].

SUMOization

DRP1 is SUMO-ized, which causes the modified DRP1 to be released back into the cytoplasm and inhibits mitochondrial division, while the de-SUMOized protein SENP3 de-SUMOizes DRP1, which, in turn, restores DRP1 function, promotes DRP1 translocation to the OMM, increases the time DRP1 spends on the OMM, and thus promotes mitochondrial division, cytochrome C release, and cell death [117,118,119]. Dual-specificity phosphatase 6 (DUSP6) is a dephosphorylase. DUSP6 can dephosphorylate DRP1 Ser-616, and the K234 site of DUSP6 itself can be modified by SUMOization. DUSP6 can become stable after being modified [120].

O-GlcNAcylation

Protein glycosylation is the covalent attachment of monosaccharides or glycans to select residues of the target protein, and glycosylation occurs mainly on serine and threonine residues [121]. O-GlcNAcylation is mainly regulated by two proteins, OGT and OGA. The OGT catalyzes the O-linked N-acetylglucosamine (O-GlcNAc), while OGA removes the O-GlcNAc residue. Threonine residues on DRP1, such as Thr-585 and Thr-586, are able to undergo glycosylation [122]. The ability to promote DRP1 glycosylation by inhibiting OGA has been demonstrated to promote its mitochondrial fragmentation and damage cells [121].

Acetylation

DRP1 is able to be acetylated at K642. K642 is located within GED, which regulates DRP1 oligomerization and GTPase activity. K642 acetylation increases the stability of DRP1, and Drp1 acetylation at K642 promotes phosphorylation of Drp1 at S616, thereby promoting mitochondrial fission [123].

S-Nitrosylation

S-Nitrosylation is a post-translational modification of the free sulfhydryl group in cysteine by nitric oxide, a process that is reversible, and nitric oxide is able to covalently bind to the target protein to form S-nitrosothiol (SNO) [124]. Many proteins in mammals are S-Nitrosylated. S-Nitrosylation plays an important role in cell proliferation, apoptosis, cell migration, and the tumor microenvironment [125,126,127]. DRP1 is able to be S-Nitrosylated at the 644 site of cysteine (Cys644), and the modified DRP1 is overactivated with increased translocation, promoting mitochondrial fission and fragmentation of the mitochondrial network, ultimately leading to cell death [128,129]. It has also been shown that S-Nitrosylation of DRP1 may regulate DRP1-S616 phosphorylation, thereby promoting mitochondrial fission [130].

4. FIS1- and DRP1-Dependent Mitochondrial Dynamics in Kidney Disease

4.1. Acute Kidney Injury (AKI)

AKI is now considered to be a public health problem with a very high human impact and, to some extent, can contribute to progression of chronic kidney disease (CKD) [131]. AKI is a frequent complication in hospitalized patients [132] and exhibits high mortality and high prevalence. AKI is characterized by a strong inflammatory response in the kidneys and body circulation, and this systemic inflammatory response leads to dysfunction of other organs, in addition to often causing acidosis, electrolyte abnormalities, and infections [133]. AKI is often characterized by an increase in serum creatinine and blood urea nitrogen and a decrease in urine output [134]. In addition, if the tubular recovery is incomplete in AKI, it can lead to long-term dysfunction and, to a certain extent, can evolve into CKD. During AKI, mitochondria are often fragmented, and mitochondrial fission proteins, such as FIS1 and DRP1, show an increase. Therefore, drugs can inhibit the increase in mitochondrial fission proteins, improve the fragmentation of mitochondria, and promote the fusion of mitochondria [135]. Increased mitochondrial fission induces mitochondrial dysfunction, leading to altered renal cell function and structure, as well as loss of renal function. It is possible to restore renal function by improving mitochondrial homeostasis and function. It is expected that DRP1 and FIS1 inhibitors may restore mitochondrial and renal function in AKI models [7]. AKI is accompanied by excessive ROS production, promoting mitochondrial fission protein expression and activation, causing renal tubular cell injury, apoptosis, and necrosis [136]. Studies have indicated that drugs that eliminate ROS, such as quercetin and resveratrol, can effectively alleviate acute kidney injury [137,138].

4.2. Chronic Kidney Disease (CKD)

CKD is a relatively common disease, with a prevalence of about 10.6–13.4%. The prevalence has risen during recent decades: it shows a trend that CKD progresses less in women than in men [139]. CKD often brings about vascular endothelial dysfunction, and cardiovascular disease is the leading cause of death in CKD patients [140]. In contrast, studies have demonstrated that aortic endothelial cells in CKD mice exhibit increased DRP1 expression and decreased MFN2 levels, and that pharmacological inhibition of DRP1 expression improves endothelial dysfunction [141,142]. Chronic renal failure (CRF), characterized by glomerulosclerosis and interstitial fibrosis, is a common end stage of various chronic kidney diseases (CKDs). TGF-β1 is an early biomarker of fibrosis. Downregulation of mitochondrial fusion proteins OPA1 and MFN2 and upregulation of fission protein DRP1 are often observed in cells with high TGF-β1 expression. The imbalance of mitochondrial dynamics plays an important role in tissue pathogenesis, so it is of great interest to block the effect of TGF-β1 on mitochondrial-dynamics-related proteins by drugs [143]. During progression of AKI to CKD, there is often an increase in mitochondrial fission and a decrease in mitochondrial fusion, and disturbances in mitochondrial dynamics promote development of AKI to CKD. When DRP1 and FIS1 are reduced, progression of AKI to CKD can be effectively mitigated [95]. It is documented that mitochondrial dysfunction may affect the severity of CKD, and persistent mitochondrial dysfunction leads to persistent tubular damage. This may also affect the kidney’s recovery from AKI and further progression to CKD [144]. Since increased FIS1/DRP1 expression in CKD can cause subsequent mitochondrial dysfunction, inhibiting FIS1/DRP1 expression is critical in improving and preventing CKD. Increasing evidence indicates that elevated ROS levels play a major role in CKD pathogenesis. Elevated intracellular ROS levels can cause lipid, DNA, and protein oxidation, as well as mitochondrial fragmentation, resulting in cellular damage [145]. Therefore, pharmacological treatment to reduce ROS is also required to improve CKD.

4.3. Diabetic Kidney Disease (DKD)

DKD has become the major cause of chronic kidney disease worldwide, and the rise in the prevalence of diabetic nephropathy is similar to the dramatic increase in the global prevalence of diabetes [146,147]. Diabetic nephropathy is the strongest predictor of mortality in diabetic patients [148]. Renal tubular injury is an early feature of DKD; renal tubular cells have abundant mitochondria. Mitochondrial fragmentation is an important pathogenic feature of renal tubular cell injury, and FIS1 and DRP1 play an important role in mitochondrial fission. In renal tubular cells with DKD, mitochondria are fragmented and FIS1 is increasing, while downregulation of FIS1 can improve mitochondrial morphology and reduce apoptosis of renal cells [149,150]. It has been shown that pharmacological inhibition of DRP1 expression and protection of mitochondria from excessive division can effectively stop progression of DKD [99]. DKD is accompanied by mitochondrial dysfunction, a decrease in renal function due to tubular damage, and mitochondrial dysfunction contributes to DKD progression and development [151]. When FIS1/DRP1 is decreased, increasing MFN2, a mitochondrial-fusion-related protein, can improve mitochondrial dysfunction [152]. Diabetic nephropathy models exhibit high ROS, which induces inflammation, fibrosis, and activation of mitochondrial fission proteins. Berberine (BBR) can effectively reduce ROS and DRP1 expression to protect the foot cells in diabetic nephropathy [99].

5. Drugs Targeting FIS1 and DRP1 and Their Role in Kidney Disease

FIS1 and DRP1 play pivotal roles in mitochondrial fission. Therefore, using drugs targeting FIS1 and DRP1 is important in improving kidney disease. Cisplatin is a chemotherapeutic agent used in treatment of cancer, but its use is often accompanied by AKI [153]. Meanwhile, curcumin can target FIS1 and prevent elevation of FIS1 as well as prevent decrease in mitochondrial fusion protein; the protective and preventive role of curcumin in cisplatin-induced AKI cannot be ignored [135]. Emodin is an anthraquinone derivative that significantly prevents increase in DRP1 expression and, thus, promotes reduced renal cell injury in AKI [154], and magnesium stigmasterate B plays a similar protective role in AKI by targeting DRP1 to renal cells [155]. High glucose often causes fragmentation of the mitochondrial network and cell death. Empagliflozin is a drug that slows progression of renal disease in diabetic patients. It was shown that, in the presence of high glucose, 100 nM of empagliflozin was effective in reducing the expression of DRP1 and 500 nM of empagliflozin was effective in reducing the expression of FIS1, in addition to the upregulation of mitochondrial fusion proteins and the downregulation of ROS exhibited by empagliflozin [156]. BBR is an isoquinoline alkaloid found in Chinese herbal medicines and widely used in treatment of diabetes. BBR protects renal cells by targeting DRP1 and inhibiting DRP1-mediated mitochondrial fission [99]. Mdivi1, a mitochondrial fission inhibitor, inhibits DRP1 expression and is effective in improving and preventing renal fibrosis after Mdivi1 administration [157], and has cytoprotective effects on renal epithelial cells in an animal model of acute kidney injury [158]. Polydatin (PD) is a resveratrol glycoside that protects kidney function in patients with diabetic nephropathy, and PD is able to inhibit podocyte injury by suppressing DRP1 expression and mitochondrial fragmentation [159]. Formononetin (FMN) is a novel isoflavonoid constituent isolated from Astragalus membranaceus; it can reduce mitochondrial fission protein, increase mitochondrial fusion protein, and improve mitochondrial damage in diabetic nephropathy [150]. P110 is an inhibitor of DRP1 and FIS1 interaction and can improve mitochondrial damage by blocking the interaction between the two fissions [160].

6. Summary and Outlook

Mitochondria are organelles with diverse roles and are involved in a variety of biological functions. Mitochondria can regulate other organelles, and, in turn, other organelles can regulate the morphological functions of mitochondria. In the past, attention was often focused on the energetics of mitochondria, but, as research progressed, it became clear that the powerful role of mitochondria is not limited to energy production. Mitochondria are also capable of determining survival of cells, which is often associated with mitochondrial dynamics. Mitochondrial dynamics consist mainly of fission, fusion, and cristae remodeling. Abnormal dysfunction in one of the three is often associated with a poor outcome. Pathological increases in mitochondrial fission are often accompanied by changes in the permeability of the outer cell membrane, which subsequently trigger a series of programmed cell deaths. However, a moderate increase in mitochondrial fission can be beneficial for axonal cells. For elimination of mitochondrial fusion, which is lethal to the cell and the organism, a moderate increase in fusion can contribute to cell survival and can repair damaged mitochondria to some extent. Remodeling of the cristae also plays an important role in the cell as they contain many energy-producing proteins and proteins that regulate cell death, such as cytochrome C. When the opening of the cristae expands, the contents of the cristae flow out, leading to a decrease in energy production and cell death.
The kidney is a very important body organ that serves as a “filter” of the body. The mitochondrial content of the kidney is quite high. Mitochondrial and kidney dysfunction caused by increased mitochondrial fission are complementary and form a vicious cycle. When the fission protein FIS1/DRP1 is reduced by drugs, it can have a protective effect on the kidney. Mitochondrial fission proteins undergo different post-translational modifications of proteins and often produce different fruitful effects, so a full understanding of their mechanisms of action is important for future prevention as well as treatment of kidney diseases.

Author Contributions

L.Q. conceived and drafted this manuscript. S.X. revised and approved the final manuscript. All authors have read and agreed to the published version of the manuscript.

Funding

The work was supported by the National Key Research and Development Program of China (Grant No. 2018YFC1801204).

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

Not applicable.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Koch, R.E.; Josefson, C.C.; Hill, G.E. Mitochondrial function, ornamentation, and immunocompetence. Biol. Rev. Camb. Philos. Soc. 2017, 92, 1459–1474. [Google Scholar] [CrossRef] [PubMed]
  2. Pfanner, N.; Warscheid, B.; Wiedemann, N. Mitochondrial proteins: From biogenesis to functional networks. Nat. Rev. Mol. Cell Biol. 2019, 20, 267–284. [Google Scholar] [CrossRef]
  3. Jin, J.-Y.; Wei, X.-X.; Zhi, X.-L.; Wang, X.-H.; Meng, D. Drp1-dependent mitochondrial fission in cardiovascular disease. Acta Pharmacol. Sin. 2021, 42, 655–664. [Google Scholar] [CrossRef] [PubMed]
  4. Horbay, R.; Bilyy, R. Mitochondrial dynamics during cell cycling. Apoptosis 2016, 21, 1327–1335. [Google Scholar] [CrossRef] [PubMed]
  5. Qin, S.-L.; Deng, J.; Lou, D.-D.; Yu, W.-F.; Pei, J.; Guan, Z.-Z. The decreased expression of mitofusin-1 and increased fission-1 together with alterations in mitochondrial morphology in the kidney of rats with chronic fluorosis may involve elevated oxidative stress. J. Trace Elem. Med. Biol. 2015, 29, 263–268. [Google Scholar] [CrossRef]
  6. Lee, Y.-J.; Jeong, S.-Y.; Karbowski, M.; Smith, C.L.; Youle, R.J. Roles of the Mammalian Mitochondrial Fission and Fusion Mediators Fis1, Drp1, and Opa1 in Apoptosis. Mol. Biol. Cell 2004, 15, 5001–5011. [Google Scholar] [CrossRef] [Green Version]
  7. Bhargava, P.; Schnellmann, R.G. Mitochondrial energetics in the kidney. Nat. Rev. Nephrol. 2017, 13, 629–646. [Google Scholar] [CrossRef]
  8. Ahmad, A.A.; Draves, S.O.; Rosca, M. Mitochondria in Diabetic Kidney Disease. Cells 2021, 10, 2945. [Google Scholar] [CrossRef]
  9. Xu, T.; Dong, Q.; Luo, Y.; Liu, Y.; Gao, L.; Pan, Y.; Zhang, D. Porphyromonas gingivalis infection promotes mitochondrial dysfunction through Drp1-dependent mitochondrial fission in endothelial cells. Int. J. Oral Sci. 2021, 13, 28. [Google Scholar] [CrossRef]
  10. Liu, X.; Xu, C.; Xu, L.; Li, X.; Sun, H.; Xue, M.; Li, T.; Yu, X.; Sun, B.; Chen, L. Empagliflozin improves diabetic renal tubular injury by alleviating mitochondrial fission via AMPK/SP1/PGAM5 pathway. Metabolism 2020, 111, 154334. [Google Scholar] [CrossRef]
  11. Wai, T.; Langer, T. Mitochondrial Dynamics and Metabolic Regulation. Trends Endocrinol. Metab. 2016, 27, 105–117. [Google Scholar] [CrossRef] [PubMed]
  12. Giacomello, M.; Pyakurel, A.; Glytsou, C.; Scorrano, L. The cell biology of mitochondrial membrane dynamics. Nat. Rev. Mol. Cell Biol. 2020, 21, 204–224. [Google Scholar] [CrossRef] [PubMed]
  13. Vásquez-Trincado, C.; García-Carvajal, I.; Pennanen, C.; Parra, V.; Hill, J.A.; Rothermel, B.A.; Lavandero, S. Mitochondrial dynamics, mitophagy and cardiovascular disease. J. Physiol. 2016, 594, 509–525. [Google Scholar] [CrossRef] [PubMed]
  14. Tilokani, L.; Nagashima, S.; Paupe, V.; Prudent, J. Mitochondrial dynamics: Overview of molecular mechanisms. Essays Biochem. 2018, 62, 341–360. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  15. Meyer, J.N.; Leuthner, T.C.; Luz, A.L. Mitochondrial fusion, fission, and mitochondrial toxicity. Toxicology 2017, 391, 42–53. [Google Scholar] [CrossRef]
  16. Chan, D.C. Mitochondrial Dynamics and Its Involvement in Disease. Annu. Rev. Pathol. 2020, 15, 235–259. [Google Scholar] [CrossRef] [Green Version]
  17. Adebayo, M.; Singh, S.; Singh, A.P.; Dasgupta, S. Mitochondrial fusion and fission: The fine-tune balance for cellular homeostasis. FASEB J. 2021, 35, e21620. [Google Scholar] [CrossRef]
  18. Cipolat, S.; Rudka, T.; Hartmann, D.; Costa, V.; Serneels, L.; Craessaerts, K.; Metzger, K.; Frezza, C.; Annaert, W.; D’Adamio, L.; et al. Mitochondrial Rhomboid PARL Regulates Cytochrome c Release during Apoptosis via OPA1-Dependent Cristae Remodeling. Cell 2006, 126, 163–175. [Google Scholar] [CrossRef]
  19. Cogliati, S.; Frezza, C.; Soriano, M.E.; Varanita, T.; Quintana-Cabrera, R.; Corrado, M.; Cipolat, S.; Costa, V.; Casarin, A.; Gomes, L.C.; et al. Mitochondrial Cristae Shape Determines Respiratory Chain Supercomplexes Assembly and Respiratory Efficiency. Cell 2013, 155, 160–171. [Google Scholar] [CrossRef] [Green Version]
  20. Friedman, J.R.; Lackner, L.L.; West, M.; DiBenedetto, J.R.; Nunnari, J.; Voeltz, G.K. ER Tubules Mark Sites of Mitochondrial Division. Science 2011, 334, 358–362. [Google Scholar] [CrossRef]
  21. Wong, Y.C.; Ysselstein, D.; Krainc, D. Mitochondria–lysosome contacts regulate mitochondrial fission via RAB7 GTP hydrolysis. Nature 2018, 554, 382–386. [Google Scholar] [CrossRef] [PubMed]
  22. Nagashima, S.; Tábara, L.-C.; Tilokani, L.; Paupe, V.; Anand, H.; Pogson, J.H.; Zunino, R.; McBride, H.M.; Prudent, J. Golgi-derived PI (4) P-containing vesicles drive late steps of mitochondrial division. Science 2020, 367, 1366–1371. [Google Scholar] [CrossRef] [PubMed]
  23. Korobova, F.; Ramabhadran, V.; Higgs, H.N. An Actin-Dependent Step in Mitochondrial Fission Mediated by the ER-Associated Formin INF2. Science 2013, 339, 464–467. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  24. Manor, U.; Bartholomew, S.; Golani, G.; Christenson, E.; Kozlov, M.; Higgs, H.; Spudich, J.; Lippincott-Schwartz, J. A mitochondria-anchored isoform of the actin-nucleating spire protein regulates mitochondrial division. eLife 2015, 4, e08828. [Google Scholar] [CrossRef]
  25. Sabouny, R.; Shutt, T.E. Reciprocal Regulation of Mitochondrial Fission and Fusion. Trends Biochem. Sci. 2020, 45, 564–577. [Google Scholar] [CrossRef] [PubMed]
  26. Liu, Y.J.; McIntyre, R.L.; Janssens, G.E.; Houtkooper, R.H. Mitochondrial fission and fusion: A dynamic role in aging and potential target for age-related disease. Mech. Ageing Dev. 2020, 186, 111212. [Google Scholar] [CrossRef]
  27. Han, H.; Tan, J.; Wang, R.; Wan, H.; He, Y.; Yan, X.; Guo, J.; Gao, Q.; Li, J.; Shang, S.; et al. PINK1 phosphorylates Drp1(S616) to regulate mitophagy-independent mitochondrial dynamics. EMBO Rep. 2020, 21, e48686. [Google Scholar] [CrossRef]
  28. Pernas, L.; Scorrano, L. Mito-Morphosis: Mitochondrial Fusion, Fission, and Cristae Remodeling as Key Mediators of Cellular Function. Annu. Rev. Physiol. 2016, 78, 505–531. [Google Scholar] [CrossRef]
  29. Yu, R.; Jin, S.; Lendahl, U.; Nistér, M.; Zhao, J. Human Fis1 regulates mitochondrial dynamics through inhibition of the fusion machinery. EMBO J. 2019, 38, e99748. [Google Scholar] [CrossRef]
  30. Scheffer, D.D.L.; Garcia, M.A.A.; Lee, M.L.; Mochly-Rosen, D.; Ferreira, J.C.B. Mitochondrial Fusion, Fission, and Mitophagy in Cardiac Diseases: Challenges and Therapeutic Opportunities. Antioxid. Redox Signal. 2022, 36, 844–863. [Google Scholar] [CrossRef]
  31. Anand, R.; Wai, T.; Baker, M.J.; Kladt, N.; Schauss, A.C.; Rugarli, E.; Langer, T. The i-AAA protease YME1L and OMA1 cleave OPA1 to balance mitochondrial fusion and fission. J. Cell Biol. 2014, 204, 919–929. [Google Scholar] [CrossRef] [PubMed]
  32. Bertholet, A.; Delerue, T.; Millet, A.; Moulis, M.; David, C.; Daloyau, M.; Arnauné-Pelloquin, L.; Davezac, N.; Mils, V.; Miquel, M.; et al. Mitochondrial fusion/fission dynamics in neurodegeneration and neuronal plasticity. Neurobiol. Dis. 2016, 90, 3–19. [Google Scholar] [CrossRef] [PubMed]
  33. Liu, X.; Weaver, D.; Shirihai, O.; Hajnoczky, G. Mitochondrial ‘kiss-and-run’: Interplay between mitochondrial motility and fusion-fission dynamics. EMBO J. 2009, 28, 3074–3089. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  34. Gao, S.; Hu, J. Mitochondrial Fusion: The Machineries In and Out. Trends Cell Biol. 2021, 31, 62–74. [Google Scholar] [CrossRef] [PubMed]
  35. Galloway, C.A.; Yoon, Y. Mitochondrial Morphology in Metabolic Diseases. Antioxid. Redox Signal. 2013, 19, 415–430. [Google Scholar] [CrossRef] [Green Version]
  36. Lu, Y.; Chen, L.; Ye, J.; Chen, C.; Zhou, Y.; Li, K.; Zhang, Z.; Peng, M. Surgery/Anesthesia disturbs mitochondrial fission/fusion dynamics in the brain of aged mice with postoperative delirium. Aging 2020, 12, 844–865. [Google Scholar] [CrossRef]
  37. Koshiba, T.; Detmer, S.A.; Kaiser, J.T.; Chen, H.; McCaffery, J.M.; Chan, D.C. Structural Basis of Mitochondrial Tethering by Mitofusin Complexes. Science 2004, 305, 858–862. [Google Scholar] [CrossRef] [Green Version]
  38. De Brito, O.M.; Scorrano, L. Mitofusin 2 tethers endoplasmic reticulum to mitochondria. Nature 2008, 456, 605–610. [Google Scholar] [CrossRef]
  39. Filadi, R.; Greotti, E.; Turacchio, G.; Luini, A.; Pozzan, T.; Pizzo, P. Mitofusin 2 ablation increases endoplasmic reticulum–mitochondria coupling. Proc. Natl. Acad. Sci. USA 2015, 112, E2174–E2181. [Google Scholar] [CrossRef] [Green Version]
  40. Nan, J.; Hu, H.; Sun, Y.; Zhu, L.; Wang, Y.; Zhong, Z.; Zhao, J.; Zhang, N.; Wang, Y.; Wang, Y.; et al. TNFR2 Stimulation Promotes Mitochondrial Fusion via Stat3- and NF-kB-Dependent Activation of OPA1 Expression. Circ. Res. 2017, 121, 392–410. [Google Scholar] [CrossRef]
  41. Wai, T.; García-Prieto, J.; Baker, M.J.; Merkwirth, C.; Benit, P.; Rustin, P.; Rupérez, F.J.; Barbas, C.; Ibañez, B.; Langer, T. Imbalanced OPA1 processing and mitochondrial fragmentation cause heart failure in mice. Science 2015, 350, aad0116. [Google Scholar] [CrossRef] [PubMed]
  42. Zhang, Y.; Wang, Y.; Xu, J.; Tian, F.; Hu, S.; Chen, Y.; Fu, Z. Melatonin attenuates myocardial ischemia-reperfusion injury via improving mitochondrial fusion/mitophagy and activating the AMPK-OPA1 signaling pathways. J. Pineal Res. 2019, 66, e12542. [Google Scholar] [CrossRef] [PubMed]
  43. Liu, C.; Han, Y.; Gu, X.; Li, M.; Du, Y.; Feng, N.; Li, J.; Zhang, S.; Maslov, L.N.; Wang, G.; et al. Paeonol promotes Opa1-mediated mitochondrial fusion via activating the CK2α-Stat3 pathway in diabetic cardiomyopathy. Redox Biol. 2021, 46, 102098. [Google Scholar] [CrossRef] [PubMed]
  44. Frezza, C.; Cipolat, S.; de Brito, O.M.; Micaroni, M.; Beznoussenko, G.V.; Rudka, T.; Bartoli, D.; Polishuck, R.S.; Danial, N.N.; De Strooper, B.; et al. OPA1 Controls Apoptotic Cristae Remodeling Independently from Mitochondrial Fusion. Cell 2006, 126, 177–189. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  45. Mannella, C.A. Structure and dynamics of the mitochondrial inner membrane cristae. Biochim. Biophys. Acta BBA Mol. Cell Res. 2006, 1763, 542–548. [Google Scholar] [CrossRef] [Green Version]
  46. Iwasawa, R.; Mahul-Mellier, A.-L.; Datler, C.; Pazarentzos, E.; Grimm, S. Fis1 and Bap31 bridge the mitochondria-ER interface to establish a platform for apoptosis induction. EMBO J. 2011, 30, 556–568. [Google Scholar] [CrossRef] [Green Version]
  47. Lewis, S.C.; Uchiyama, L.F.; Nunnari, J. ER-mitochondria contacts couple mtDNA synthesis with mitochondrial division in human cells. Science 2016, 353, aaf5549. [Google Scholar] [CrossRef] [Green Version]
  48. Boutry, M.; Kim, P.K. ORP1L mediated PI(4)P signaling at ER-lysosome-mitochondrion three-way contact contributes to mitochondrial division. Nat. Commun. 2021, 12, 5354. [Google Scholar] [CrossRef]
  49. Wong, Y.C.; Kim, S.; Peng, W.; Krainc, D. Regulation and Function of Mitochondria–Lysosome Membrane Contact Sites in Cellular Homeostasis. Trends Cell Biol. 2019, 29, 500–513. [Google Scholar] [CrossRef]
  50. Jackson, C.L. Activators and Effectors of the Small G Protein Arf1 in Regulation of Golgi Dynamics During the Cell Division Cycle. Front. Cell Dev. Biol. 2018, 6, 29. [Google Scholar] [CrossRef]
  51. Rasmussen, M.L.; Robertson, G.L.; Gama, V. Break on Through: Golgi-Derived Vesicles Aid in Mitochondrial Fission. Cell Metab. 2020, 31, 1047–1049. [Google Scholar] [CrossRef] [PubMed]
  52. Yang, C.; Svitkina, T.M. Ultrastructure and dynamics of the actin−myosin II cytoskeleton during mitochondrial fission. Nat. Cell Biol. 2019, 21, 603–613. [Google Scholar] [CrossRef] [PubMed]
  53. Scherz-Shouval, R.; Elazar, Z. Regulation of autophagy by ROS: Physiology and pathology. Trends Biochem. Sci. 2011, 36, 30–38. [Google Scholar] [CrossRef] [PubMed]
  54. Hu, J.; Zhang, Y.; Jiang, X.; Zhang, H.; Gao, Z.; Li, Y.; Fu, R.; Li, L.; Li, J.; Cui, H.; et al. ROS-mediated activation and mitochondrial translocation of CaMKII contributes to Drp1-dependent mitochondrial fission and apoptosis in triple-negative breast cancer cells by isorhamnetin and chloroquine. J. Exp. Clin. Cancer Res. 2019, 38, 225. [Google Scholar] [CrossRef] [PubMed]
  55. Aranda-Rivera, A.K.; Cruz-Gregorio, A.; Aparicio-Trejo, O.E.; Pedraza-Chaverri, J. Mitochondrial Redox Signaling and Oxidative Stress in Kidney Diseases. Biomolecules 2021, 11, 1144. [Google Scholar] [CrossRef] [PubMed]
  56. Tang, S.; Ye, S.; Ma, Y.; Liang, Y.; Liang, N.; Xiao, F. Clusterin alleviates Cr(VI)-induced mitochondrial apoptosis in L02 hepatocytes via inhibition of Ca2+-ROS-Drp1-mitochondrial fission axis. Ecotoxicol. Environ. Saf. 2020, 205, 111326. [Google Scholar] [CrossRef]
  57. Huang, Q.; Zhan, L.; Cao, H.; Li, J.; Lyu, Y.; Guo, X.; Zhang, J.; Ji, L.; Ren, T.; An, J.; et al. Increased mitochondrial fission promotes autophagy and hepatocellular carcinoma cell survival through the ROS-modulated coordinated regulation of the NFKB and TP53 pathways. Autophagy 2016, 12, 999–1014. [Google Scholar] [CrossRef] [Green Version]
  58. Clerkin, J.S.; Naughton, R.; Quiney, C.; Cotter, T.G. Mechanisms of ROS modulated cell survival during carcinogenesis. Cancer Lett. 2008, 266, 30–36. [Google Scholar] [CrossRef]
  59. Tsushima, K.; Bugger, H.; Wende, A.; Soto, J.; Jenson, G.A.; Tor, A.R.; McGlauflin, R.; Kenny, H.C.; Zhang, Y.; Souvenir, R.; et al. Mitochondrial Reactive Oxygen Species in Lipotoxic Hearts Induce Post-Translational Modifications of AKAP121, DRP1, and OPA1 That Promote Mitochondrial Fission. Circ. Res. 2018, 122, 58–73. [Google Scholar] [CrossRef]
  60. Wu, K.; Mao, Y.Y.; Chen, Q.; Zhang, B.; Zhang, S.; Wu, H.J.; Li, Y. Hypoxia-induced ROS promotes mitochondrial fission and cisplatin chemosensitivity via HIF-1alpha/Mff regulation in head and neck squamous cell carcinoma. Cell Oncol. 2021, 44, 1167–1181. [Google Scholar] [CrossRef]
  61. Kleele, T.; Rey, T.; Winter, J.; Zaganelli, S.; Mahecic, D.; Lambert, H.P.; Ruberto, F.P.; Nemir, M.; Wai, T.; Pedrazzini, T.; et al. Distinct fission signatures predict mitochondrial degradation or biogenesis. Nature 2021, 593, 435–439. [Google Scholar] [CrossRef] [PubMed]
  62. Wang, B.; Nguyen, M.; Chang, N.C.; Shore, G.C. Fis1, Bap31 and the kiss of death between mitochondria and endoplasmic reticulum. EMBO J. 2011, 30, 451–452. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  63. Haileselassie, B.; Mukherjee, R.; Joshi, A.U.; Napier, B.A.; Massis, L.M.; Ostberg, N.P.; Queliconi, B.B.; Monack, D.; Bernstein, D.; Mochly-Rosen, D. Drp1/Fis1 interaction mediates mitochondrial dysfunction in septic cardiomyopathy. J. Mol. Cell. Cardiol. 2019, 130, 160–169. [Google Scholar] [CrossRef] [PubMed]
  64. Suzuki, M.; Jeong, S.-Y.; Karbowski, M.; Youle, R.J.; Tjandra, N. The Solution Structure of Human Mitochondria Fission Protein Fis1 Reveals a Novel TPR-like Helix Bundle. J. Mol. Biol. 2003, 334, 445–458. [Google Scholar] [CrossRef] [Green Version]
  65. Zhang, Y.; Chan, D.C. Structural basis for recruitment of mitochondrial fission complexes by Fis1. Proc. Natl. Acad. Sci. USA 2007, 104, 18526–18530. [Google Scholar] [CrossRef] [Green Version]
  66. Jofuku, A.; Ishihara, N.; Mihara, K. Analysis of functional domains of rat mitochondrial Fis1, the mitochondrial fission-stimulating protein. Biochem. Biophys. Res. Commun. 2005, 333, 650–659. [Google Scholar] [CrossRef]
  67. D’Andrea, L.D.; Regan, L. TPR proteins: The versatile helix. Trends Biochem. Sci. 2003, 28, 655–662. [Google Scholar] [CrossRef]
  68. Yu, Y.; Peng, X.-D.; Qian, X.-J.; Zhang, K.-M.; Huang, X.; Chen, Y.-H.; Li, Y.-T.; Feng, G.-K.; Zhang, H.-L.; Xu, X.-L.; et al. Fis1 phosphorylation by Met promotes mitochondrial fission and hepatocellular carcinoma metastasis. Signal Transduct. Target. Ther. 2021, 6, 401. [Google Scholar] [CrossRef]
  69. Rovira-Llopis, S.; Bañuls, C.; Diaz-Morales, N.; Hernandez-Mijares, A.; Rocha, M.; Victor, V.M. Mitochondrial dynamics in type 2 diabetes: Pathophysiological implications. Redox Biol. 2017, 11, 637–645. [Google Scholar] [CrossRef]
  70. Losón, O.C.; Song, Z.; Chen, H.; Chan, D.C. Fis1, Mff, MiD49, and MiD51 mediate Drp1 recruitment in mitochondrial fission. Mol. Biol. Cell 2013, 24, 659–667. [Google Scholar] [CrossRef]
  71. Joshi, A.U.; Ebert, A.E.; Haileselassie, B.; Mochly-Rosen, D. Drp1/Fis1-mediated mitochondrial fragmentation leads to lysosomal dysfunction in cardiac models of Huntington’s disease. J. Mol. Cell. Cardiol. 2019, 127, 125–133. [Google Scholar] [CrossRef] [PubMed]
  72. Mukherjee, R.; Tompkins, C.A.; Ostberg, N.P.; Joshi, A.U.; Massis, L.M.; Vijayan, V.; Gera, K.; Monack, D.; Cornell, T.T.; Hall, M.W.; et al. Drp1/Fis1-Dependent Pathologic Fission and Associated Damaged Extracellular Mitochondria Contribute to Macrophage Dysfunction in Endotoxin Tolerance. Crit. Care Med. 2022, 50, e504–e515. [Google Scholar] [CrossRef]
  73. Chakrabarti, R.; Higgs, H.N. Revolutionary view of two ways to split a mitochondrion. Nature 2021, 593, 346–347. [Google Scholar] [CrossRef] [PubMed]
  74. Wang, S.; Zhu, H.; Li, R.; Mui, D.; Toan, S.; Chang, X.; Zhou, H. DNA-PKcs interacts with and phosphorylates Fis1 to induce mitochondrial fragmentation in tubular cells during acute kidney injury. Sci. Signal. 2022, 15, eabh1121. [Google Scholar] [CrossRef] [PubMed]
  75. Wei, Q.-J.; Xu, H.; Guan, N.; Ren, Y.-L.; Liu, X.-Y.; Wu, G.-H.; Zhu, S.-N. Overproduction of Mitochondrial Fission Proteins in Membranous Nephropathy in Children. Kidney Blood Press. Res. 2018, 43, 1927–1934. [Google Scholar] [CrossRef]
  76. Yi, J.; Liao, J.; Bai, T.; Wang, B.; Yangzom, C.; Ahmed, Z.; Mehmood, K.; Abbas, R.Z.; Li, Y.; Tang, Z.; et al. Battery wastewater induces nephrotoxicity via disordering the mitochondrial dynamics. Chemosphere 2022, 303, 135018. [Google Scholar] [CrossRef]
  77. Kato, M.; Abdollahi, M.; Tunduguru, R.; Tsark, W.; Chen, Z.; Wu, X.; Wang, J.; Chen, Z.B.; Lin, F.M.; Lanting, L.; et al. miR-379 deletion ameliorates features of diabetic kidney disease by enhancing adaptive mitophagy via FIS1. Commun. Biol. 2021, 4, 30. [Google Scholar] [CrossRef]
  78. Bilbrough, T.; Piemontese, E.; Seitz, O. Dissecting the role of protein phosphorylation: A chemical biology toolbox. Chem. Soc. Rev. 2022, 51, 5691–5730. [Google Scholar] [CrossRef]
  79. Hornbeck, P.V.; Zhang, B.; Murray, B.; Kornhauser, J.M.; Latham, V.; Skrzypek, E. PhosphoSitePlus, 2014: Mutations, PTMs and recalibrations. Nucleic Acids Res. 2015, 43, D512–D520. [Google Scholar] [CrossRef] [Green Version]
  80. Zou, R.; Shi, W.; Qiu, J.; Na Zhou, N.; Na Du, N.; Zhou, H.; Chen, X.; Ma, L. Empagliflozin attenuates cardiac microvascular ischemia/reperfusion injury through improving mitochondrial homeostasis. Cardiovasc. Diabetol. 2022, 21, 106. [Google Scholar] [CrossRef]
  81. Popovic, D.; Vucic, D.; Dikic, I. Ubiquitination in disease pathogenesis and treatment. Nat. Med. 2014, 20, 1242–1253. [Google Scholar] [CrossRef] [PubMed]
  82. Swatek, K.N.; Komander, D. Ubiquitin modifications. Cell Res. 2016, 26, 399–422. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  83. Tang, J.; Hu, Z.; Tan, J.; Yang, S.; Zeng, L. Parkin Protects against Oxygen-Glucose Deprivation/Reperfusion Insult by Promoting Drp1 Degradation. Oxidative Med. Cell. Longev. 2016, 2016, 8474303. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  84. Nardin, A.; Schrepfer, E.; Ziviani, E. Counteracting PINK/Parkin Deficiency in the Activation of Mitophagy: A Potential Therapeutic Intervention for Parkinson’s Disease. Curr. Neuropharmacol. 2016, 14, 250–259. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  85. Heo, J.-M.; Ordureau, A.; Swarup, S.; Paulo, J.A.; Shen, K.; Sabatini, D.M.; Harper, J.W. RAB7A phosphorylation by TBK1 promotes mitophagy via the PINK-PARKIN pathway. Sci. Adv. 2018, 4, eaav0443. [Google Scholar] [CrossRef] [Green Version]
  86. 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]
  87. Nakamura, N.; Kimura, Y.; Tokuda, M.; Honda, S.; Hirose, S. MARCH-V is a novel mitofusin 2- and Drp1-binding protein able to change mitochondrial morphology. EMBO Rep. 2006, 7, 1019–1022. [Google Scholar] [CrossRef] [Green Version]
  88. Park, Y.-Y.; Lee, S.; Karbowski, M.; Neutzner, A.; Youle, R.J.; Cho, H. Loss of MARCH5 mitochondrial E3 ubiquitin ligase induces cellular senescence through dynamin-related protein 1 and mitofusin 1. J. Cell Sci. 2010, 123, 619–626. [Google Scholar] [CrossRef] [Green Version]
  89. Chang, H.-M.; Yeh, E.T.H. SUMO: From Bench to Bedside. Physiol. Rev. 2020, 100, 1599–1619. [Google Scholar] [CrossRef]
  90. Wilkinson, K.A.; Guo, C. Iron chelation promotes mitophagy through SENP3-mediated deSUMOylation of FIS1. Autophagy 2022, 18, 1743–1745. [Google Scholar] [CrossRef]
  91. Waters, E.; Wilkinson, K.; Harding, A.L.; Carmichael, R.; Robinson, D.; Colley, H.; Guo, C. The SUMO protease SENP3 regulates mitochondrial autophagy mediated by Fis1. EMBO Rep. 2022, 23, e48754. [Google Scholar] [CrossRef] [PubMed]
  92. Rardin, M.J.; Newman, J.C.; Held, J.M.; Cusack, M.P.; Sorensen, D.J.; Li, B.; Schilling, B.; Mooney, S.D.; Kahn, C.R.; Verdin, E.; et al. Label-free quantitative proteomics of the lysine acetylome in mitochondria identifies substrates of SIRT3 in metabolic pathways. Proc. Natl. Acad. Sci. USA 2013, 110, 6601–6606. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  93. Lombard, D.B.; Alt, F.W.; Cheng, H.-L.; Bunkenborg, J.; Streeper, R.S.; Mostoslavsky, R.; Kim, J.; Yancopoulos, G.; Valenzuela, D.; Murphy, A.; et al. Mammalian Sir2 Homolog SIRT3 Regulates Global Mitochondrial Lysine Acetylation. Mol. Cell. Biol. 2007, 27, 8807–8814. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  94. Baeza, J.; Smallegan, M.J.; Denu, J.M. Mechanisms and Dynamics of Protein Acetylation in Mitochondria. Trends Biochem. Sci. 2016, 41, 231–244. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  95. Cheng, L.; Yang, X.; Jian, Y.; Liu, J.; Ke, X.; Chen, S.; Yang, D.; Yang, D. SIRT3 deficiency exacerbates early-stage fibrosis after ischaemia-reperfusion-induced AKI. Cell. Signal. 2022, 93, 110284. [Google Scholar] [CrossRef]
  96. Meng, G.; Liu, J.; Liu, S.; Song, Q.; Liu, L.; Xie, L.; Han, Y.; Ji, Y. Hydrogen sulfide pretreatment improves mitochondrial function in myocardial hypertrophy via a SIRT3-dependent manner. J. Cereb. Blood Flow Metab. 2018, 175, 1126–1145. [Google Scholar] [CrossRef] [Green Version]
  97. Fröhlich, C.; Grabiger, S.; Schwefel, D.; Faelber, K.; Rosenbaum, E.; Mears, J.; Rocks, O.; Daumke, O. Structural insights into oligomerization and mitochondrial remodelling of dynamin 1-like protein. EMBO J. 2013, 32, 1280–1292. [Google Scholar] [CrossRef] [Green Version]
  98. Smirnova, E.; Griparic, L.; Shurland, D.-L.; van der Bliek, A.M. Dynamin-related Protein Drp1 Is Required for Mitochondrial Division in Mammalian Cells. Mol. Biol. Cell 2001, 12, 2245–2256. [Google Scholar] [CrossRef] [Green Version]
  99. Qin, X.; Zhao, Y.; Gong, J.; Huang, W.; Su, H.; Yuan, F.; Fang, K.; Wang, D.; Li, J.; Zou, X.; et al. Berberine Protects Glomerular Podocytes via Inhibiting Drp1-Mediated Mitochondrial Fission and Dysfunction. Theranostics 2019, 9, 1698–1713. [Google Scholar] [CrossRef]
  100. Wang, J.; Zhu, P.; Li, R.; Ren, J.; Zhou, H. Fundc1-dependent mitophagy is obligatory to ischemic preconditioning-conferred renoprotection in ischemic AKI via suppression of Drp1-mediated mitochondrial fission. Redox Biol. 2020, 30, 101415. [Google Scholar] [CrossRef]
  101. Qi, Z.; Huang, Z.; Xie, F.; Chen, L. Dynamin-related protein 1: A critical protein in the pathogenesis of neural system dysfunctions and neurodegenerative diseases. J. Cell. Physiol. 2019, 234, 10032–10046. [Google Scholar] [CrossRef] [PubMed]
  102. Serasinghe, M.N.; Chipuk, J.E. Mitochondrial Fission in Human Diseases. Antibiotics 2017, 240, 159–188. [Google Scholar] [CrossRef]
  103. Yu, W.; Wang, X.; Zhao, J.; Liu, R.; Liu, J.; Wang, Z.; Peng, J.; Wu, H.; Zhang, X.; Long, Z.; et al. Stat2-Drp1 mediated mitochondrial mass increase is necessary for pro-inflammatory differentiation of macrophages. Redox Biol. 2020, 37, 101761. [Google Scholar] [CrossRef]
  104. Qu, C.; Yang, W.; Kan, Y.; Zuo, H.; Wu, M.; Zhang, Q.; Wang, H.; Wang, D.; Chen, J. RhoA/ROCK Signaling Regulates Drp1-Mediated Mitochondrial Fission During Collective Cell Migration. Front. Cell Dev. Biol. 2022, 10, 882581. [Google Scholar] [CrossRef] [PubMed]
  105. Brand, C.S.; Tan, V.P.; Brown, J.H.; Miyamoto, S. RhoA regulates Drp1 mediated mitochondrial fission through ROCK to protect cardiomyocytes. Cell. Signal. 2018, 50, 48–57. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  106. Zhu, J.; Zhang, G.; Song, Z.; Xiang, X.; Shu, S.; Liu, Z.; Yang, D.; Wei, Q.; Dong, Z. Protein Kinase C-delta Mediates Kidney Tubular Injury in Cold Storage-Associated Kidney Transplantation. J. Am. Soc. Nephrol. 2020, 31, 1050–1065. [Google Scholar] [CrossRef]
  107. Feng, W.; Wang, J.; Yan, X.; Zhang, Q.; Chai, L.; Wang, Q.; Shi, W.; Chen, Y.; Liu, J.; Qu, Z.; et al. ERK/Drp1-dependent mitochondrial fission contributes to HMGB1-induced autophagy in pulmonary arterial hypertension. Cell Prolif. 2021, 54, e13048. [Google Scholar] [CrossRef]
  108. Xu, S.; Wang, P.; Zhang, H.; Gong, G.; Cortes, N.G.; Zhu, W.; Yoon, Y.; Tian, R.; Wang, W. CaMKII induces permeability transition through Drp1 phosphorylation during chronic beta-AR stimulation. Nat. Commun. 2016, 7, 13189. [Google Scholar] [CrossRef] [Green Version]
  109. Rong, R.; Xia, X.; Peng, H.; Li, H.; You, M.; Liang, Z.; Yao, F.; Yao, X.; Xiong, K.; Huang, J.; et al. Cdk5-mediated Drp1 phosphorylation drives mitochondrial defects and neuronal apoptosis in radiation-induced optic neuropathy. Cell Death Dis. 2020, 11, 720. [Google Scholar] [CrossRef]
  110. Jung, J.-U.; Ravi, S.; Lee, D.W.; McFadden, K.; Kamradt, M.L.; Toussaint, L.G.; Sitcheran, R. NIK/MAP3K14 Regulates Mitochondrial Dynamics and Trafficking to Promote Cell Invasion. Curr. Biol. 2016, 26, 3288–3302. [Google Scholar] [CrossRef]
  111. Torres, G.; Morales, P.E.; García-Miguel, M.; Norambuena-Soto, I.; Cartes-Saavedra, B.; Vidal-Peña, G.; Moncada-Ruff, D.; Sanhueza-Olivares, F.; Martín, A.S.; Chiong, M. Glucagon-like peptide-1 inhibits vascular smooth muscle cell dedifferentiation through mitochondrial dynamics regulation. Biochem. Pharmacol. 2016, 104, 52–61. [Google Scholar] [CrossRef] [Green Version]
  112. Du, J.; Li, H.; Song, J.; Wang, T.; Dong, Y.; Zhan, A.; Li, Y.; Liang, G. AMPK Activation Alleviates Myocardial Ischemia-Reperfusion Injury by Regulating Drp1-Mediated Mitochondrial Dynamics. Front. Pharmacol. 2022, 13, 862204. [Google Scholar] [CrossRef] [PubMed]
  113. Cherok, E.; Xu, S.; Li, S.; Das, S.; Meltzer, W.A.; Zalzman, M.; Wang, C.; Karbowski, M. Novel regulatory roles of Mff and Drp1 in E3 ubiquitin ligase MARCH5–dependent degradation of MiD49 and Mcl1 and control of mitochondrial dynamics. Mol. Biol. Cell 2017, 28, 396–410. [Google Scholar] [CrossRef]
  114. Karbowski, M.; Neutzner, A.; Youle, R.J. The mitochondrial E3 ubiquitin ligase MARCH5 is required for Drp1 dependent mitochondrial division. J. Cell Biol. 2007, 178, 71–84. [Google Scholar] [CrossRef] [PubMed]
  115. Yamada, T.; Murata, D.; Adachi, Y.; Itoh, K.; Kameoka, S.; Igarashi, A.; Kato, T.; Araki, Y.; Huganir, R.L.; Dawson, T.M.; et al. Mitochondrial Stasis Reveals p62-Mediated Ubiquitination in Parkin-Independent Mitophagy and Mitigates Nonalcoholic Fatty Liver Disease. Cell Metab. 2018, 28, 588–604.e5. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  116. Yamada, T.; Dawson, T.M.; Yanagawa, T.; Iijima, M.; Sesaki, H. SQSTM1/p62 promotes mitochondrial ubiquitination independently of PINK1 and PRKN/parkin in mitophagy. Autophagy 2019, 15, 2012–2018. [Google Scholar] [CrossRef] [PubMed]
  117. Anderson, C.; Blackstone, C. SUMO wrestling with Drp1 at mitochondria. EMBO J. 2013, 32, 1496–1498. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  118. De Souza, A.C.G.; Prediger, R.D.; Cimarosti, H. SUMO-regulated mitochondrial function in Parkinson’s disease. J. Neurochem. 2016, 137, 673–686. [Google Scholar] [CrossRef] [Green Version]
  119. Guo, C.; Wilkinson, K.A.; Evans, A.J.; Rubin, P.P.; Henley, J.M. SENP3-mediated deSUMOylation of Drp1 facilitates interaction with Mff to promote cell death. Sci. Rep. 2017, 7, 43811. [Google Scholar] [CrossRef] [Green Version]
  120. Ma, R.; Ma, L.; Weng, W.; Wang, Y.; Liu, H.; Guo, R.; Gao, Y.; Tu, J.; Xu, T.-L.; Cheng, J.; et al. DUSP6 SUMOylation protects cells from oxidative damage via direct regulation of Drp1 dephosphorylation. Sci. Adv. 2020, 6, eaaz0361. [Google Scholar] [CrossRef]
  121. Gawlowski, T.; Suarez, J.; Scott, B.; Torres-Gonzalez, M.; Wang, H.; Schwappacher, R.; Han, X.; Yates, J.R., 3rd; Hoshijima, M.; Dillmann, W. Modulation of dynamin-related protein 1 (DRP1) function by increased O-linked-beta-N-acetylglucosamine modification (O-GlcNAc) in cardiac myocytes. J. Biol. Chem. 2012, 287, 30024–30034. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  122. Park, S.J.; Bae, J.E.; Jo, D.S.; Kim, J.B.; Park, N.Y.; Fang, J.; Jung, Y.K.; Jo, D.G.; Cho, D.H. Increased O-GlcNAcylation of Drp1 by amyloid-beta promotes mitochondrial fission and dysfunction in neuronal cells. Mol. Brain. 2021, 14, 6. [Google Scholar] [CrossRef] [PubMed]
  123. Hu, Q.; Zhang, H.; Cortés, N.G.; Wu, D.; Wang, P.; Zhang, J.; Mattison, J.A.; Smith, E.; Bettcher, L.F.; Wang, M.; et al. Increased Drp1 Acetylation by Lipid Overload Induces Cardiomyocyte Death and Heart Dysfunction. Circ. Res. 2020, 126, 456–470. [Google Scholar] [CrossRef] [PubMed]
  124. Sharma, V.; Fernando, V.; Letson, J.; Walia, Y.; Zheng, X.; Fackelman, D.; Furuta, S. S-Nitrosylation in Tumor Microenvironment. Int. J. Mol. Sci. 2021, 22, 4600. [Google Scholar] [CrossRef]
  125. Ehrenfeld, P.; Cordova, F.; Duran, W.N.; Sanchez, F.A. S-nitrosylation and its role in breast cancer angiogenesis and metastasis. Nitric Oxide 2019, 87, 52–59. [Google Scholar] [CrossRef]
  126. Benhar, M.; Stamler, J.S. A central role for S-nitrosylation in apoptosis. Nat. Cell Biol. 2005, 7, 645–646. [Google Scholar] [CrossRef]
  127. Hess, D.T.; Matsumoto, A.; Kim, S.-O.; Marshall, H.E.; Stamler, J.S. Protein S-nitrosylation: Purview and parameters. Nat. Rev. Mol. Cell Biol. 2005, 6, 150–166. [Google Scholar] [CrossRef]
  128. Zhao, Q.-F.; Yu, J.-T.; Tan, L. S-Nitrosylation in Alzheimer’s disease. Mol. Neurobiol. 2015, 51, 268–280. [Google Scholar] [CrossRef]
  129. Cho, D.H.; Nakamura, T.; Fang, J.; Cieplak, P.; Godzik, A.; Gu, Z.; Lipton, S.A. S-nitrosylation of Drp1 mediates beta-amyloid-related mitochondrial fission and neuronal injury. Science 2009, 324, 102–105. [Google Scholar] [CrossRef] [Green Version]
  130. Lee, D.-S.; Kim, J.-E. PDI-mediated S-nitrosylation of DRP1 facilitates DRP1-S616 phosphorylation and mitochondrial fission in CA1 neurons. Cell Death Dis. 2018, 9, 869. [Google Scholar] [CrossRef]
  131. Singbartl, K.; Kellum, J.A. AKI in the ICU: Definition, epidemiology, risk stratification, and outcomes. Kidney Int. 2012, 81, 819–825. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  132. Vijayan, A. Tackling AKI: Prevention, timing of dialysis and follow-up. Nat. Rev. Nephrol. 2021, 17, 87–88. [Google Scholar] [CrossRef] [PubMed]
  133. Hoste, E.A.; De Corte, W. Clinical Consequences of Acute Kidney Injury. Contrib. Nephrol. 2011, 174, 56–64. [Google Scholar] [CrossRef] [PubMed]
  134. Yang, Y.; Song, M.; Liu, Y.; Liu, H.; Sun, L.; Peng, Y.; Liu, F.; Venkatachalam, M.A.; Dong, Z. Renoprotective approaches and strategies in acute kidney injury. Pharmacol. Ther. 2016, 163, 58–73. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  135. Ortega-Domínguez, B.; Aparicio-Trejo, O.E.; García-Arroyo, F.E.; León-Contreras, J.C.; Tapia, E.; Molina-Jijón, E.; Hernández-Pando, R.; Sanchez-Lozada, L.-G.; Barrera-Oviedo, D.; Pedraza-Chaverri, J. Curcumin prevents cisplatin-induced renal alterations in mitochondrial bioenergetics and dynamic. Food Chem. Toxicol. 2017, 107, 373–385. [Google Scholar] [CrossRef] [PubMed]
  136. Zhao, M.; Wang, Y.; Li, L.; Liu, S.; Wang, C.; Yuan, Y.; Yang, G.; Chen, Y.; Cheng, J.; Lu, Y.; et al. Mitochondrial ROS promote mitochondrial dysfunction and inflammation in ischemic acute kidney injury by disrupting TFAM-mediated mtDNA maintenance. Theranostics 2021, 11, 1845–1863. [Google Scholar] [CrossRef]
  137. Wang, Y.; Quan, F.; Cao, Q.; Lin, Y.; Yue, C.; Bi, R.; Cui, X.; Yang, H.; Yang, Y.; Birnbaumer, L.; et al. Quercetin alleviates acute kidney injury by inhibiting ferroptosis. J. Adv. Res. 2021, 28, 231–243. [Google Scholar] [CrossRef]
  138. Kitada, M.; Koya, D. Renal Protective Effects of Resveratrol. Oxidative Med. Cell. Longev. 2013, 2013, 568093. [Google Scholar] [CrossRef] [Green Version]
  139. Swartling, O.; Rydell, H.; Stendahl, M.; Segelmark, M.; Lagerros, Y.T.; Evans, M. CKD Progression and Mortality Among Men and Women: A Nationwide Study in Sweden. Am. J. Kidney Dis. 2021, 78, 190–199.e1. [Google Scholar] [CrossRef]
  140. Kahn, M.R.; Robbins, M.J.; Kim, M.C.; Fuster, V. Management of cardiovascular disease in patients with kidney disease. Nat. Rev. Cardiol. 2013, 10, 261–273. [Google Scholar] [CrossRef]
  141. Su, H.; Liu, B.; Chen, H.; Zhang, T.; Huang, T.; Liu, Y.; Wang, C.; Ma, Q.; Wang, Q.; Lv, Z.; et al. LncRNA ANRIL mediates endothelial dysfunction through BDNF downregulation in chronic kidney disease. Cell Death Dis. 2022, 13, 661. [Google Scholar] [CrossRef] [PubMed]
  142. Huang, M.; Wei, R.; Wang, Y.; Su, T.; Li, P.; Chen, X. The uremic toxin hippurate promotes endothelial dysfunction via the activation of Drp1-mediated mitochondrial fission. Redox Biol. 2018, 16, 303–313. [Google Scholar] [CrossRef] [PubMed]
  143. Sun, L.; Yuan, Q.; Xu, T.; Yao, L.; Feng, J.; Ma, J.; Wang, L.; Lu, C.; Wang, D. Pioglitazone Improves Mitochondrial Function in the Remnant Kidney and Protects against Renal Fibrosis in 5/6 Nephrectomized Rats. Front. Pharmacol. 2017, 8, 545. [Google Scholar] [CrossRef] [Green Version]
  144. Ryan, A.S. Role of Skeletal Muscle Mitochondrial Dysfunction in CKD. Clin. J. Am. Soc. Nephrol. 2020, 15, 912–913. [Google Scholar] [CrossRef]
  145. Irazabal, M.V.; Torres, V.E. Reactive Oxygen Species and Redox Signaling in Chronic Kidney Disease. Cells 2020, 9, 1342. [Google Scholar] [CrossRef] [PubMed]
  146. Alicic, R.Z.; Rooney, M.T.; Tuttle, K.R. Diabetic Kidney Disease: Challenges, Progress, and Possibilities. Clin. J. Am. Soc. Nephrol. 2017, 12, 2032–2045. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  147. Mendis, S.; Davis, S.; Norrving, B. Organizational update: The world health organization global status report on noncommunicable diseases 2014; one more landmark step in the combat against stroke and vascular disease. Stroke 2015, 46, e121–e122. [Google Scholar] [CrossRef]
  148. Reidy, K.; Kang, H.M.; Hostetter, T.; Susztak, K. Molecular mechanisms of diabetic kidney disease. J. Clin. Investig. 2014, 124, 2333–2340. [Google Scholar] [CrossRef]
  149. Zhan, M.; Usman, I.; Yu, J.; Ruan, L.; Bian, X.; Yang, J.; Yang, S.; Sun, L.; Kanwar, Y.S. Perturbations in mitochondrial dynamics by p66Shc lead to renal tubular oxidative injury in human diabetic nephropathy. Clin. Sci. 2018, 132, 1297–1314. [Google Scholar] [CrossRef]
  150. Huang, Q.; Chen, H.; Yin, K.; Shen, Y.; Lin, K.; Guo, X.; Zhang, X.; Wang, N.; Xin, W.; Xu, Y.; et al. Formononetin Attenuates Renal Tubular Injury and Mitochondrial Damage in Diabetic Nephropathy Partly via Regulating Sirt1/PGC-1alpha Pathway. Front. Pharmacol. 2022, 13, 901234. [Google Scholar] [CrossRef]
  151. Wei, P.Z.; Szeto, C.C. Mitochondrial dysfunction in diabetic kidney disease. Clin. Chim. Acta 2019, 496, 108–116. [Google Scholar] [CrossRef] [PubMed]
  152. Tagaya, M.; Kume, S.; Yasuda-Yamahara, M.; Kuwagata, S.; Yamahara, K.; Takeda, N.; Tanaka, Y.; Chin-Kanasaki, M.; Nakae, Y.; Yokoi, H.; et al. Inhibition of mitochondrial fission protects podocytes from albumin-induced cell damage in diabetic kidney disease. Biochim. Et Biophys. Acta Mol. Basis Dis. 2022, 1868, 166368. [Google Scholar] [CrossRef]
  153. Ozkok, A.; Edelstein, C.L. Pathophysiology of cisplatin-induced acute kidney injury. BioMed Res. Int. 2014, 2014, 967826. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  154. Wang, Y.; Liu, Q.; Cai, J.; Wu, P.; Wang, D.; Shi, Y.; Huyan, T.; Su, J.; Li, X.; Wang, Q.; et al. Emodin prevents renal ischemia-reperfusion injury via suppression of CAMKII/DRP1-mediated mitochondrial fission. Eur. J. Pharmacol. 2022, 916, 174603. [Google Scholar] [CrossRef]
  155. Shen, D.; Guo, M.; Geng, X.; Yu, J.; Zhang, Z.; Lin, J.; Lin, P.; Ding, X.; Xu, X. Magnesium Lithospermate B Protects Against Cisplatin-Induced Acute Kidney Injury via Alleviating Mitochondrial Dysfunction. Drug Des. Dev. Ther. 2022, 16, 2293–2304. [Google Scholar] [CrossRef] [PubMed]
  156. Lee, W.-C.; Chau, Y.-Y.; Ng, H.-Y.; Chen, C.-H.; Wang, P.-W.; Liou, C.-W.; Lin, T.-K.; Chen, J.-B. Empagliflozin Protects HK-2 Cells from High Glucose-Mediated Injuries via a Mitochondrial Mechanism. Cells 2019, 8, 1085. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  157. Wang, Y.; Lu, M.; Xiong, L.; Fan, J.; Zhou, Y.; Li, H.; Peng, X.; Zhong, Z.; Wang, Y.; Huang, F.; et al. Drp1-mediated mitochondrial fission promotes renal fibroblast activation and fibrogenesis. Cell Death Dis. 2020, 11, 29. [Google Scholar] [CrossRef] [Green Version]
  158. Brooks, C.; Wei, Q.; Cho, S.-G.; Dong, Z. Regulation of mitochondrial dynamics in acute kidney injury in cell culture and rodent models. J. Clin. Investig. 2009, 119, 1275–1285. [Google Scholar] [CrossRef]
  159. Ni, Z.; Tao, L.; Xiaohui, X.; Zelin, Z.; Jiangang, L.; Zhao, S.; Weikang, H.; Hongchao, X.; Qiujing, W.; Xin, L. Polydatin impairs mitochondria fitness and ameliorates podocyte injury by suppressing Drp1 expression. J. Cell. Physiol. 2017, 232, 2776–2787. [Google Scholar] [CrossRef] [Green Version]
  160. Haileselassie, B.; Joshi, A.U.; Minhas, P.S.; Mukherjee, R.; Andreasson, K.I.; Mochly-Rosen, D. Mitochondrial dysfunction mediated through dynamin-related protein 1 (Drp1) propagates impairment in blood brain barrier in septic encephalopathy. J. Neuroinflamm. 2020, 17, 36. [Google Scholar] [CrossRef]
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Figure 1. The structure of mitochondria. OMM: mitochondrial outer membrane. IMM: inner mitochondrial membrane. Cristae: mitochondrial inner membrane is depressed inward to form cristae. Matrix: internal space wrapped by the inner mitochondrial membrane. IMS: the space between the outer mitochondrial membrane and the inner mitochondrial membrane.
Figure 1. The structure of mitochondria. OMM: mitochondrial outer membrane. IMM: inner mitochondrial membrane. Cristae: mitochondrial inner membrane is depressed inward to form cristae. Matrix: internal space wrapped by the inner mitochondrial membrane. IMS: the space between the outer mitochondrial membrane and the inner mitochondrial membrane.
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Figure 2. The process of mitochondrial fission and fusion. (a): The mitochondrial fission process and related proteins, mitochondrial outer membrane proteins FIS1, Mid49, Mid51, and MFF, are capable of recruiting DRP1 from the cytoplasm to the mitochondrial outer membrane. (b): The mitochondrial fusion process and related proteins, the mitochondrial outer membrane proteins MFN1 and MFN2, are responsible for the fusion of the outer mitochondrial membrane, and the mitochondrial inner membrane protein OPA1 is responsible for the fusion of the inner mitochondrial membrane.
Figure 2. The process of mitochondrial fission and fusion. (a): The mitochondrial fission process and related proteins, mitochondrial outer membrane proteins FIS1, Mid49, Mid51, and MFF, are capable of recruiting DRP1 from the cytoplasm to the mitochondrial outer membrane. (b): The mitochondrial fusion process and related proteins, the mitochondrial outer membrane proteins MFN1 and MFN2, are responsible for the fusion of the outer mitochondrial membrane, and the mitochondrial inner membrane protein OPA1 is responsible for the fusion of the inner mitochondrial membrane.
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Figure 3. Cristae remodeling. (a): Under normal conditions, L-OPA1 and S-OPA1 are able to form oligomers to maintain the structure and function of the cristae. (b): The cristae remodel, the opening of the cristae becomes larger, and the contents of the cristae are released.
Figure 3. Cristae remodeling. (a): Under normal conditions, L-OPA1 and S-OPA1 are able to form oligomers to maintain the structure and function of the cristae. (b): The cristae remodel, the opening of the cristae becomes larger, and the contents of the cristae are released.
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Figure 4. Interactions between mitochondria and other organelles promote mitochondrial fission. (a): The ER-bound INF2 and mitochondrial Spire1C induce actin nucleation and polymerization at mitochondria–ER contact sites. (b): The RAB7-GTP protein on the lysosome can bind to an unknown protein on the outer mitochondrial membrane to form a mitochondrial–lysosomal contact, and the mitochondrial outer membrane protein FIS1 is able to recruit TBC1D15, which is able to hydrolyze RAB7-GTP to RAB7-GDP and unbind it. (c): Golgi-derived vesicles containing PI(4)P contribute to mitochondrial division.
Figure 4. Interactions between mitochondria and other organelles promote mitochondrial fission. (a): The ER-bound INF2 and mitochondrial Spire1C induce actin nucleation and polymerization at mitochondria–ER contact sites. (b): The RAB7-GTP protein on the lysosome can bind to an unknown protein on the outer mitochondrial membrane to form a mitochondrial–lysosomal contact, and the mitochondrial outer membrane protein FIS1 is able to recruit TBC1D15, which is able to hydrolyze RAB7-GTP to RAB7-GDP and unbind it. (c): Golgi-derived vesicles containing PI(4)P contribute to mitochondrial division.
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Figure 5. Schematic diagram of the FIS1 structure. TPR, a1–a6 are six a-helices connected by short rings; residues Val11-Ala27, Lys32-Val43, Asn48-Leu62, Lys67-Arg83, Tyr87-Thr100, Asn105-Lys120 form α1, α2, α3, α4, α5, α6, respectively. The TMD region is responsible for the location of FIS1.
Figure 5. Schematic diagram of the FIS1 structure. TPR, a1–a6 are six a-helices connected by short rings; residues Val11-Ala27, Lys32-Val43, Asn48-Leu62, Lys67-Arg83, Tyr87-Thr100, Asn105-Lys120 form α1, α2, α3, α4, α5, α6, respectively. The TMD region is responsible for the location of FIS1.
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Figure 6. Schematic diagram of the DRP1 structure. GTPase: highly conserved N-terminal GTPase domain. Middle: helical middle domain. Variable: variable domain (also known as insert B). GED: a C-terminal GTPase effector domain.
Figure 6. Schematic diagram of the DRP1 structure. GTPase: highly conserved N-terminal GTPase domain. Middle: helical middle domain. Variable: variable domain (also known as insert B). GED: a C-terminal GTPase effector domain.
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Table
Table 1. Post-translational modifications of FIS1.
Table 1. Post-translational modifications of FIS1.
Type of ModificationPositionUpstream MoleculesEffects
PhosphorylationY38METPhosphorylation
/DNA-PKcsPhosphorylation
Ubiquitination/ParkinUbiquitination
/MARCH5Ubiquitination
SUMOylationK149SENP3DeSUMOylation
Acetylation/SIRT3DeAcetylation
Table
Table 2. Post-translational modifications of DRP1.
Table 2. Post-translational modifications of DRP1.
Type of ModificationPositionUpstream MoleculesEffects
PhosphorylationSer-616Stat2Phosphorylation
PKCδPhosphorylation
ERK1/2Phosphorylation
CaMKIIPhosphorylation
Cdk5Phosphorylation
ROCKPhosphorylation
DUSP6DePhosphorylation
Ser-637PKAThe specific role of S637 phosphorylation
results from diverse internal and external
parameters
PKD
CaN
AMPK
Ubiquitination/ParkinUbiquitination
/MARCH5Ubiquitination
/SQSTM1/P62Ubiquitination
SUMOylation/SENP3DeSUMOylation
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Qin, L.; Xi, S. The role of Mitochondrial Fission Proteins in Mitochondrial Dynamics in Kidney Disease. Int. J. Mol. Sci. 2022, 23, 14725. https://doi.org/10.3390/ijms232314725

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Qin L, Xi S. The role of Mitochondrial Fission Proteins in Mitochondrial Dynamics in Kidney Disease. International Journal of Molecular Sciences. 2022; 23(23):14725. https://doi.org/10.3390/ijms232314725

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Qin, Lingyu, and Shuhua Xi. 2022. "The role of Mitochondrial Fission Proteins in Mitochondrial Dynamics in Kidney Disease" International Journal of Molecular Sciences 23, no. 23: 14725. https://doi.org/10.3390/ijms232314725

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