The impact of cellular senescence on aging skeletal muscle

Abstract

Skeletal muscle is a highly plastic tissue that relies on its resident muscle stem cell population, known as satellite cells (MuSC), for its timely repair and regeneration. During aging, there is a decline in muscle regenerative capacity that is largely attributed to the loss of MuSC content and function. These aberrations are thought to contribute to the aging-related decline in skeletal muscle mass and strength. Cellular senescence, which is characterized by a state of irreversible cell cycle arrest and the presence of a senescence-associated secretory phenotype (SASP), has emerged as a potential factor in the dysfunction of MuSCs with aging. Much effort has recently been made to examine the detrimental effects of senescence on skeletal muscle as well as identify therapeutic approaches to selectively eliminate these cells and improve the aging phenotype. Here, we discuss the current understanding of aging-related MuSC impairments and the underlying mechanisms that link cellular senescence to the decline in muscle regenerative capacity.

1 Introduction

As humans age, we experience declines in overall health and organ-specific function throughout our bodies. Certain factors, such as genomic instability, stem cell exhaustion, and mitochondrial dysfunction, contribute to these progressive and inevitable changes (López-Otín et al., 2023). Skeletal muscle, as a highly dynamic and metabolic tissue, is particularly susceptible to the progressive decline in molecular and cellular function that occurs with advanced age, which could eventually lead to sarcopenia and frailty. These diseases cause a significant loss of independence and are major risk factors for developing aging-associated comorbidities (Cruz-Jentoft and Sayer, 2019; Pacifico et al., 2020; Sasaki and Fukumoto, 2022). Several mechanisms have been previously identified that actively contribute to muscle dysfunction with aging, but recently, research into cellular senescence has revealed a potentially large role for this fundamental biological process (Granic et al., 2023; Muñoz-Espín and Serrano, 2014). Cellular senescence, the irreversible arrest of cell proliferation, is a physiological stress response and a known hallmark of aging. When cells are unable to adequately respond to damaging stimuli, internal homeostatic machinery can force the cell into a state of senescence or premature apoptosis (Collado et al., 2007; Van Deursen, 2014). Numerous studies over the last decade have linked senescence to aging-related muscle impairments, indicating that our understanding of how cellular aging drives these deficits is still limited and requires further investigation (Zhang X. et al., 2022; Englund et al., 2021; He et al., 2021). This review aims to discuss the unique biological processes involved with cellular senescence, and how these features can influence skeletal muscle dynamics during periods of damage and regeneration. Specifically, we will highlight the known mechanisms that contribute to the aging-related dysfunction of muscle stem cells, the essential hallmarks of senescence and the SASP, the current evidence implicating senescence in skeletal muscle aging, and the implications of clearing senescent cells from the muscle microenvironment.

2 Muscle stem cells and aging

Under healthy, homeostatic conditions, muscle stem cells or satellite cells (MuSCs) are quiescent until activated in response to muscle damage, after which they differentiate to repair and regenerate the injured tissue. The naturally quiescent status of MuSCs makes them especially susceptible to the accumulation of intracellular damage that occurs during aging, ultimately resulting in a decrease in both MuSC number and function (Sousa-Victor and Muñoz-Cánoves, 2016). These detriments have led to impairments in the regenerative capacity of aged muscle (Conboy and Rando, 2005). While the change in MuSC characteristics is well documented in aged humans and animals, there is still much debate about the extent to which the MuSC perturbations with aging contribute to sarcopenia. Previous work has shown that MuSC depletion in sedentary mice does not affect muscle size during aging despite lower regenerative capacity (Fry et al., 2015; Keefe et al., 2015). On the other hand, there is evidence that MuSC content is associated with the regulation of muscle mass during aging. One group found that the depletion of MuSCs limits the hypertrophic growth response to lifelong physical activity in aged mice (Englund et al., 2020). Furthermore, it is well known that MuSCs in extraocular muscles are maintained in aging and muscle dystrophy, which is accompanied by the sparing of these muscles from the associated muscle wasting (Formicola et al., 2014; Kaminski et al., 1992). More recently, published work implicated the fibrogenic conversion of MuSCs as a significant component of sarcopenia and demonstrated that melatonin treatment replenishes the MuSC pool and mitigates the loss of muscle mass and strength in aged mice (Zhu et al., 2024). Unfortunately, there is still no definitive consensus on whether satellite cells significantly contribute to sarcopenia in humans. There is inherently a relationship between MuSCs and sarcopenia, but whether the loss or dysfunction of these cells substantially contributes to the progressive decline of skeletal muscle remains to be seen.

2.1 Mechanisms of aging-related MuSC dysfunction

The decline in MuSC content in old muscle tends to occur primarily in type II-associated MuSCs, often correlating with the substantial atrophy of type II myofibres observed with advancing age (Verdijk et al., 2007; Verdijk et al., 2014). Several mechanisms have been proposed as contributing to this loss, primarily revolving around the concept of stem cell exhaustion (Sousa-Victor et al., 2021; Ancel et al., 2021). The aged MuSC niche contains elevated levels of fibroblast growth factor (FGF), which has the unfortunate effect of driving a subset of unstimulated MuSCs to leave their quiescent state and lose their self-renewing capacity (Chakkalakal et al., 2012; Pawl et al., 2017). This is particularly detrimental in aged muscle because any damaging stimulus would be accompanied by a failure to replenish the basal MuSC pool and result in lower MuSC content throughout the muscle. Moreover, research conducted in both rodents and humans has shown that aged MuSCs are more susceptible to apoptosis than their young counterparts (Fulle et al., 2013; Jejurikar et al., 2006). Taken together, these data imply that decreases in MuSC content with aging are linked to a loss of quiescence, diminished self-renewal, and elevated cell death.

While there is a discrepancy in the field regarding the implication that diminished MuSC content significantly contributes to sarcopenia, it is possible that the functional detriments of aged MuSCs may augment the aging-associated pathology of skeletal muscle. Several molecular and metabolic perturbations contribute to the decline of MuSC function in advanced age. When healthy cells accumulate damaged organelles and components, they activate processes like autophagy to remove these materials and restore homeostasis. Like many other organs and tissues, MuSCs experience impairments in autophagy with aging, which causes a significant decline in regenerative capacity due to this loss of proteostasis (García-Prat et al., 2016a). Diminished autophagic clearance of damaged cellular components leads to the accumulation of intracellular debris and damaged mitochondria, which ultimately transitions MuSCs from a state of quiescence (reversible cell cycle arrest) to one of premature senescence (irreversible cell cycle arrest) or apoptosis (García-Prat et al., 2016b; White et al., 2018). This would also explain the inability of aged MuSCs to maintain quiescence and the decline in MuSC content with aging that was previously discussed. In addition to the reduced mitochondrial autophagy (mitophagy), aged MuSC also experience an imbalance in mitochondrial remodelling, resulting in a loss of oxidative phosphorylation (OXPHOS); crucially, genetically restoring OXPHOS or mitophagy in these cells enhances muscle regeneration (Hong et al., 2022). Further discussion on the mechanisms of senescence induction can be found in Section 3.

Cell cycle kinetics are also disrupted in aged MuSCs. Impaired mitophagy causes an increase in intracellular reactive oxygen species (ROS) levels, which in turn upregulates the expression of p16^INK4a, the cyclin-dependent kinase inhibitor (CDKI) (García-Prat et al., 2016b; Passos et al., 2007). Cyclins, a class of proteins involved in cell cycle progression, are implicated in normal myogenic proliferation and differentiation (Mademtzoglou and Relaix, 2022). Alterations in CyclinD1 levels have been observed in aged MuSCs, although there is very limited research on this topic (Brett et al., 2020; Kimmel et al., 2020). Moreover, the loci of p16 and p21 are more epigenetically silenced in young MuSCs compared to old (Li et al., 2015). This could explain why MuSCs in very old muscles experience a derepression of p16, which pushes them out of quiescence into irreversible cellular senescence (Sousa-Victor et al., 2014). The relationship between senescence and aging muscle satellite cells will be discussed further in the following sections. The molecular detriments described in this review are implicated in aging-associated MuSC dysfunction, but it remains unclear whether they are a direct consequence of the aging environment or if they independently develop over time and, in turn, exacerbate the aging phenotype.

2.2 Factors that influence satellite cell fate during aging

Genetic heterogeneity between MuSC populations often dictates cell fate during muscle regeneration and aging. As discussed above, the myogenic regulatory factors (MRFs) contribute to the progression of MuSC through the myogenic program. MuSCs that are Myf5^– are more stem-like and thus replenish the MuSC niche, whereas Myf5⁺ MuSCs are more committed to differentiation (Kuang et al., 2007). Cells lacking Myf5 or its MRF companion MyoD display very mild differentiation, while the genetic double knockout (dKO) of both MRFs completely impairs it (Yamamoto et al., 2018; Rudnicki et al., 1993; Megeney et al., 1996). Furthermore, aged mice with MyoD/Myf5^dKO MuSCs could not regenerate properly after injury (Yamamoto et al., 2018). Another study reported that MuSCs expressing high levels of Pax7 are more dormant, take longer to respond to injury and have lower metabolic activity than Pax7^Low MuSCs (Rocheteau et al., 2012). Cell surface markers can also represent different populations of MuSCs with distinct behaviours. CD34^High MuSCs are more stem-like and less likely to commit to myogenic differentiation than CD34^Low cells, not unlike the pattern observed with Pax7 expression (García-Prat et al., 2020). Surprisingly, the CD34^High quiescent preference is preserved during aging, with these MuSCs remaining dormant and only being activated at very advanced ages due to the elevation of pro-myogenic signalling (García-Prat et al., 2020). This is consistent with recent work that showed CD34⁺ MuSCs are persistently quiescent in culture and capable of maintaining their phenotype with very limited proliferation (Steele et al., 2024). These findings indicate that intrinsic factors, such as molecular heterogeneity, are directly implicated in the activity and stemness of MuSCs.

MuSCs can undergo transcriptomic and metabolic reprogramming based on their microenvironment (Sousa-Victor et al., 2021). Some of the earliest evidence of this utilized heterochronic parabiosis to show that exposing aged muscle to young, healthy serum improved MuSC function and restored muscle regenerative capacity (Co et al., 2005). MuSC within extraocular muscles (EOM) are molecularly distinct from their limb-derived counterparts and are preferentially spared from dysfunction during aging or muscular dystrophies (Formicola et al., 2014; Kaminski et al., 1992; Evano et al., 2020). Notably, transplanting EOM MuSCs into tibialis anterior (TA) muscles caused them to adopt a TA-like transcriptomic profile, indicating the molecular identity of these cells was primarily driven by the limb muscle MuSC niche (Evano et al., 2020). Even more drastically, previous work has demonstrated that the in vitro treatment with bone morphogenic proteins or adipogenic inducers can induce the osteogenic and adipogenic conversion of adult murine MuSCs (Asakura et al., 2001; Wada et al., 2002). These studies showcase the remarkable plasticity of these stem cells and suggest that the aging-related MuSC perturbations are more likely driven by extrinsic factors present in the muscle microenvironment rather than intrinsic defects in cellular components.

3 Cellular senescence–a primer

The first in vitro cell culture experiments occurred in the early 20th century when scientist Ross Harrison isolated and expanded nerve cells using explanted frog embryonic tissue (Har et al., 1907). The use of isolated cells, in vitro, expanded rapidly over the subsequent decades, and researchers around the world began developing techniques to isolate and maintain cells in culture and establish cell lines from animal and human tissues. One of the most significant discoveries came in 1961 when Leonard Hayflick and Paul Moorhead found that human fetal fibroblasts could undergo a finite number of population doublings before ultimately experiencing proliferative arrest (Hayflick and Moorhead, 1961). This finding challenged the current dogma that all cells were immortal and gave rise to the theory that normal cells had a finite replicative capacity, while cancer cell lines could proliferate indefinitely. Hayflick coined the term “cellular senescence” to describe the phenomenon of cell replicative arrest, and his seminal work began the study of aging mechanisms within cultured cells (Hayflick and Moorhead, 1961; Khokhlov, 2013). Today, senescence can be briefly defined as the irreversible arrest of the cell cycle in metabolically active and living cells.

3.1 Senescence and cellular aging

Aging is accompanied by a decline in health and function that impacts every organ throughout the body. Several cellular and molecular characteristics are often observed with advancing age that negatively impact tissue homeostasis, such as genomic instability, mitochondrial dysfunction, altered signalling, and stem cell exhaustion, to name a few (López-Otín et al., 2023). Many aging-related perturbations are brought about by the inability of cells to adequately respond to these stimuli, which usually forces them into either cellular senescence or apoptosis. Over time, this results in the accumulation of senescent cells across multiple organs and tissues, which can initiate or exacerbate age-related disorders (Van Deursen, 2014). While premature senescence induction can produce deleterious effects, the timely initiation of this mechanism does have a beneficial role in several biological functions, including embryonic development, wound healing, and tumour suppression (Collado et al., 2007; Demaria et al., 2014; Muñoz-Espín et al., 2013). The dual nature of cellular senescence is a prime example of the concept of antagonistic pleiotropy, which states that beneficial traits found in young organisms can become detrimental later in life (Wiley and Campisi, 2021).

The phenomenon discovered by Hayflick and Moorhead can now be more accurately termed “replicative senescence.” The underlying cellular mechanism behind this discovery was largely attributed to the gradual erosion of telomeres that occurred with each division (Bodnar et al., 1998). Telomeres, which are short repeat nucleotide sequences found at the end of chromosomes, protect against chromosomal deterioration during transcription. After every round of replication, DNA polymerases leave a few bases at the end of the telomere unreplicated, and for most cells, this results in the erosion of the telomeres with each cell cycle (Campisi, 1997). Fortunately, some cells express telomerase, a protective enzyme that adds telomeric repeats to chromosome ends and prevents DNA damage (Campisi, 1997). However, if telomeres reach a critical length, they trigger a DNA damage response (DDR) that induces replicative senescence (d’Adda di Fagagna et al., 2003).

For many years, replicative senescence was the sole focus within the field of cellular aging. Eventually, researchers began to observe that several other cellular perturbations are capable of inducing senescence independent of telomere erosion, such as mitochondrial dysfunction, epigenetic modifications, non-telomeric DNA damage, loss of proteostasis, oncogene activation, chronic inflammation, and oxidative stress (Chandeck and Mooi, 2010; Höhn et al., 2017; Miwa et al., 2022; Sidler et al., 2017; Wen and Klionsky, 2016). Even adjacent senescent cells were observed to cause paracrine senescence in nearby healthy cells by releasing pro-inflammatory factors as part of the senescence-associated secretory phenotype (SASP) (Acosta et al., 2013). For the purposes of this review, we will refer to the premature (i.e., non-replicative) senescent state as “stress-induced senescence”. Notably, several of these stressors are also considered hallmarks of aging (López-Otín et al., 2023), and the clearance of senescent cells in aged mice can extend both healthspan and lifespan (Xu et al., 2018). Taken together, this positions cellular senescence as a foundational component of age-related dyshomeostasis that is not just a byproduct of aging, but causative as well.

3.2 The intracellular senescence phenotype

Our understanding of cellular senescence has advanced greatly since the term was first introduced over 60 years ago. It is now apparent that the senescent phenotype is highly heterogeneous, and while there are several common characteristics, there is no single universal molecular senescence marker (Hernandez-Segura et al., 2017). This variability can be driven by a number of factors, such as the senescence-triggering stimuli, the cell type, or the passage of time. Here, we will discuss the molecular and structural alterations that occur within senescent cells (Figure 1).

FIGURE 1

3.2.1 DNA damage

Aging cells are exposed to a plethora of stressors that can cause DNA damage and consequently trigger the DDR. This damage can be in the form of single- or double-stranded breaks (SSB and DSB, respectively) which, if left unresolved, will lead to cellular senescence (Kumari and Jat, 2021). While there are a multitude of different stimuli that can prompt DNA damage, it is usually the p53/p21^CIP1 pathway that is initiated in response (Fumagalli et al., 2012). Persistent DDR signalling leads to p53 phosphorylation and p21 activation, which in turn inhibits cyclin-dependent kinase 2 (CDK2) (Campisi and D’Adda Di Fagagna, 2007). This causes the hypophosphorylation of retinoblastoma (RB), a tumour suppressor protein, that ultimately leads to cell cycle arrest and senescence (Chicas et al., 2010). Another CDKI, p16^INK4a, accumulates with age and is generally implicated in replicative senescence signalling. Like p21, p16 also hypophosphorylates RB to halt cell proliferation. Senescent growth arrest was traditionally thought to occur in the G1 phase of the cell cycle, but several studies have now shown that G2 exit can occur with p21-mediated DNA damage signalling (Gire and Dulić, 2015).

3.2.2 Apoptotic resistance

A key cellular mechanism present in many senescent cells is apoptotic resistance. Apoptosis is the programmed and highly regulated process of cell death. Like senescence, apoptosis is routinely initiated in response to extreme cellular stress. The mechanism that dictates which of these processes a damaged cell will experience is poorly understood, but one hypothesis is that acute DNA damage initiates apoptosis while sustained DNA damage induces senescence (Kumari and Jat, 2021). Notably, senescent cells often exhibit robust anti-apoptotic mechanisms to prolong their stability and lifespan, which could explain why these cells accumulate with age (Campisi and D’Adda Di Fagagna, 2007). A class of genes known as senescence-associated super-enhancers (SASE) have recently been linked to promoting the survival of senescent cells (Sturmlechner et al., 2022). In response to DNA damage, the SASE members Mdm2, Rnas4, and Ang act to suppress p53-mediated apoptosis and preserve cellular senescence (Sturmlechner et al., 2022). At first glance, apoptosis and senescence may seem like opposing cell fates; however, these processes work together to contribute to the dysfunction of aging tissues. In fact, the primary class of therapeutics aimed at combating cellular senescence–senolytics–target the anti-apoptotic pathways of senescent cells (see Section 5).

3.2.3 Metabolic alterations

The development of apoptosis resistance is accompanied by alterations in senescent cell metabolic activity. Common metabolic alterations include defects in OXPHOS and a transition to glycolytic energy systems. Senescence triggers the significant metabolic reprogramming of a cell, but these changes are highly heterogeneous and will vary based on the cell type and mode of senescence induction. For example, human fibroblasts induced to senescence via irradiation or replication have elevated glycolysis and reduced oxidative activity, while oncogene-induced senescent fibroblasts activate both glycolysis and OXPHOS (Takebayashi et al., 2015; James et al., 2015). Oddly, increased glycolysis has been shown to protect cells from premature senescence (Kondoh et al., 2005). While the metabolic activity of senescent cells is certainly modified, the large variability in physiological response makes it challenging to use metabolic parameters as universal senescence biomarkers. Importantly, senescent cells are also capable of metabolically reprogramming adjacent, non-senescent cells through the actions of the SASP (discussed further below) (Acosta et al., 2013).

3.2.4 Loss of proteostasis

Moreover, senescent cells experience a loss of proteostasis, primarily characterized by dysfunctions in autophagy. Senescent cells tend to accumulate dysfunctional lysosomes over time, a feature that is the basis for the senescence-associated β-galactosidase (SA-β-gal) assay (Dimri et al., 1995). These organelles are key components of autophagy as they regulate the degradation and recycling of unneeded cellular material (Yim and Mizushima, 2020). Furthermore, senescence often results in the elevated activity of mechanistic target of rapamycin complex 1 (mTORC1), which suppresses autophagy and restricts the cell’s ability to clear damaged components (Kang et al., 2011; Tai et al., 2017). Mitophagy is also presumably suppressed by the over-activation of mTORC1, which would reduce the clearance of dysfunctional mitochondria and exacerbate the proteostatic aberrations observed in senescent cells (Korolchuk et al., 2017).

3.2.5 Morphological changes

Cellular senescence often presents with several morphological changes that can be easily detected in vitro. Senescent cells generally exhibit an enlarged and abnormally shaped cell body, potentially due to the formation of actin stress fibres (Huang et al., 2022). Furthermore, senescent signalling can activate sodium channels on the plasma membranes of cells, elevating intracellular sodium concentrations (Warnier et al., 2018). This, in conjunction with the senescence-mediated upregulation of caveolin-1, ultimately results in plasma membrane destabilization (Cho et al., 2004; Chrétien et al., 2008; Dasari et al., 2006). More internally, senescent cells often have destabilized nuclei due to reduced Lamin B1 protein on the inner nuclear membrane, which causes chromatin remodelling and results in enlarged nuclei or multinucleation (Freund et al., 2012; Shimi et al., 2011). While these characteristics are readily identifiable in vitro, senescent cells in vivo usually retain a normal morphology dictated by their surrounding environment (Muñoz-Espín and Serrano, 2014). Mitochondrial structure is also severely impacted by cellular senescence. Typically, senescent cells have larger and more abundant mitochondria than their healthy counterparts due to blunted mitophagy that allows for the accumulation of older, dysfunctional organelles (Tai et al., 2017; Korolchuk et al., 2017; Hara et al., 2013). These mitochondria experience diminished membrane potential and have increased ROS production, leading to oxidative stress and further exacerbating the senescent phenotype (Passos et al., 2007).

3.3 The senescence-associated secretory phenotype (SASP)

Cellular senescence is not only detrimental to the affected cell, but also to the cellular microenvironment due to the actions of the SASP. This feature is capable of intercellular communication and signalling through the components released by the senescent cells. Traditionally, the SASP was characterized by the secretion of several protein types, such as cytokines, chemokines, growth factors and proteases (Coppé et al., 2008), but over the years, other molecules have been added to this list, including bioactive lipids, extracellular vesicles, and non-coding nucleic acids (Table 1) (Wang et al., 2024). While all of these components have been identified in the secretome of senescence cells, the exact composition of the SASP will vary based on cell type and the intracellular senescent phenotype present at that time (Coppé et al., 2010; Wiley et al., 2017; Basisty et al., 2020).

3.3.1 Protein-based factors

The most prominent and well-characterized component of the SASP is the proteins, which can be classified into three categories–soluble signalling proteins, proteases, and insoluble proteins. Soluble signalling proteins are a large source of bioactive molecules that have the potential to influence several signal transduction pathways related to tumour progression, inflammation, and other age-related diseases (Matsuda et al., 2023; Zhou et al., 2022; Ortiz-Montero et al., 2017). Notable members of this category include interleukins, chemokines, and growth factors (Wang et al., 2024; Matsuda et al., 2023; Orjalo et al., 2009; Severino et al., 2013). Proteases, which are responsible for the degradation of signalling proteins and the extracellular matrix (ECM), are also released as SASP factors (Liu and Hornsby, 2007). Lastly, insoluble proteins, such as the cell surface protein fibronectin, are often released by senescent cells, resulting in significant cytoskeletal remodelling (Chen et al., 2006).

3.3.2 Lipids and extracellular vesicles

Additional SASP components with prominent bioactive properties have also been identified. Certain lipids, such as phospholipids or oxidized fatty acids, are released by senescent cells and can promote fibrosis, inflammation, and cell cycle arrest (Narzt et al., 2021; Wiley et al., 2019; Wiley et al., 2021). Additionally, small extracellular vesicles (EVs) released by senescent cells have been shown to affect cell proliferation and apoptotic signalling (Takasugi et al., 2017; Terlecki-Zaniewicz et al., 2018). EVs contain proteins, lipids, and non-coding nucleic acids such as microRNAs (miRNA) and can regulate intercellular senescence communication (Takasugi, 2018). MiRNAs, which post-transcriptionally regulate gene expression, have often been identified as the primary drivers of EV-mediated senescence signalling (Disayabutr et al., 2016; Lee et al., 2023; Fabian et al., 2010; Valadi et al., 2007). Finally, there are several SASP components that are not classified under any of these categories but still have significant roles in regulating senescence-associated signalling. These include nitric oxide (NO) and ROS, which are produced because of the altered metabolism and oxidative stress present in senescent cells (Wang et al., 2024; Mabrouk et al., 2020).

3.3.3 Regulation of the SASP

The SASP is driven by multiple intracellular senescence signalling pathways, primarily those involved in the DDR (Wiley and Campisi, 2021; Rodier et al., 2009). While the current understanding of SASP regulation is limited, several mediators of the phenotype have been identified, including p53, p16, NF-κB, C/EBPβ, p38 MAPK, mTOR, and NOTCH (Coppé et al., 2008; Freund et al., 2011; Herranz et al., 2015; Acosta et al., 2008; Hoare et al., 2016; Buj et al., 2021). The SASP of DNA-damaged cells is primarily controlled by the transcription factors NF-κB and C/EBPβ, which regulate the release of interleukins, chemokines, and growth factors (Acosta et al., 2008; Chien et al., 2011). However, other key signalling molecules have also been implicated in SASP regulation. The depletion of p53 has been shown to increase the release of pro-inflammatory factors, while p16 suppression decreases the expression of multiple SASP components (Buj et al., 2021; Wiley et al., 2016). Moreover, p38 MAPK can trigger a SASP profile by activating NF-κB independent of the DDR, while mTOR promotes SASP expression by differentially regulating the translation of MK2 through 4EBP1 (Freund et al., 2011; Herranz et al., 2015). Finally, NOTCH1 activation drives a TGFβ-mediated secretome while inhibiting the C/EBPβ-mediated SASP (Hoare et al., 2016).

Short-term exposure to SASP factors can have beneficial effects, such as in wound healing or during embryonic development, but the presence of a chronic SASP can have major implications, especially for aging tissues (Demaria et al., 2014; Muñoz-Espín et al., 2013). Chronic SASP activity can have detrimental effects by causing the remodelling of the ECM, increasing fibrosis, or propagating apoptosis in otherwise healthy tissues (Wang et al., 2024). The SASP is not only a consequence of cellular senescence, but it also acts as a senescence inducer; secreted factors can propagate paracrine senescence on neighbouring, healthy cells (Faget et al., 2019). Furthermore, the SASP causes the rise of chemokine and cytokine levels in the cellular microenvironment, contributing to the chronic state of inflammation present in advanced age (Li et al., 2023). The targeted removal of senescent cells and the accompanying SASP improved physical function and extended the lifespan of aged mice, suggesting a promising therapeutic approach to combat aging-related dysfunction (Xu et al., 2018).

4 The pathophysiology of senescence within aged muscle

In recent years, there has been a growing interest in the potential for cellular senescence to be implicated in the aging-related perturbations of skeletal muscle. Early work by Baker et al. (2008) found that the systemic inactivation of p16 in BubR1-insufficient mice attenuated the degenerative loss of muscle mass and strength observed in these animals. Since then, there have been multiple investigations directly and indirectly examining the impact of cellular senescence on muscle physiology. There are three possible avenues through which senescence could elicit its effects on aged skeletal muscle: 1) the accumulation of senescent mononuclear cells in skeletal muscle; 2) the induced senescent phenotype of post-mitotic muscle components (i.e., myofibres and myonuclei); and 3) the detrimental effects of the SASP caused by senescent cells in other tissues (Figure 2). This section will discuss the available literature related to each of these theories and the potential that they are implicated in the aging-related dysfunction of skeletal muscle.

FIGURE 2

4.1 Accumulation of senescent mononuclear cells

4.1.1 Evidence supporting senescent cell accumulation

Senescent cells are known to accumulate in multiple tissues with aging, which is generally believed to be detrimental to the overall health and function of our bodies (Baker et al., 2008). Several studies have found evidence that senescent cell markers increase with aging in both rodent and human skeletal muscles (Zhang X. et al., 2022; Hudgins et al., 2018; Sosa et al., 2018; Da Silva et al., 2019). While most of this work examined cellular senescence in whole muscle, others have directly examined the muscle-resident mononuclear cell populations, such as in satellite cells (MuSC), the predominant muscle stem cell responsible for repair and regeneration. In aged muscle, multiple studies have shown that MuSCs express elevated levels of SA-β-gal, p16, and p21 (García-Prat et al., 2016b; Li et al., 2015; Sousa-Victor et al., 2014; Cosgrove et al., 2014; Zhu et al., 2019). While these observations suggest that MuSCs may be accumulating in skeletal muscle over time, one study did show that senescence is apparent only in extremely old (geriatric) MuSCs but not in young or old muscles, indicating that these cells might be accumulating genomic damage over time that only presents as senescence in very advanced ages (Sousa-Victor et al., 2014). Early work investigating muscle cell senescence also observed an accumulation of p16+ fibro-adipogenic progenitors (FAPs) in BubR1 progeroid mice (Baker et al., 2013). More recently, FAPs in aged muscle have been observed to have elevated expression of p16 (Zhang X. et al., 2022). Notably, this p16-positive FAP population had a transcriptional profile highly consistent with senescent gene signalling, providing compelling evidence that these cells were likely senescent (Zhang X. et al., 2022). Additionally, CD68⁺ macrophages and mesenchymal progenitor cells in the interstitium of skeletal muscle have elevated levels of p16 and γH2AX, respectively (Sugihara et al., 2018; Guzman et al., 2022). Others have detected elevated senescence markers in aged muscle cells, but these authors did not quantify the cell type, so it is not possible to know which populations are accumulating with age (Da Silva et al., 2019; Baker et al., 2016).

Several potential explanations exist for why muscle cells are experiencing elevated levels of senescence over time. Nearly 60% of MuSCs isolated from aged muscle or identified on isolated aged myofibres showed increased expression of γH2AX relative to their young counterparts, indicating that these cells are routinely exposed to DNA damage (Sinha et al., 2014). Furthermore, aged MuSCs exhibit a significant impairment of autophagy which reduces the clearance of dysfunctional organelles and causes the build-up of toxic cellular waste (García-Prat et al., 2016b). This results in the accumulation of damaged mitochondria that are constantly producing substantial amounts of ROS and thus promoting oxidative stress (Hong et al., 2022). Old MuSCs have also demonstrated a failure to suppress p16 activity and consequently experience an impaired myogenic capacity followed by senescence induction, which has been linked to the activation of p38 MAPK and the reduction of H2AK119Ub-mediated silencing (Sousa-Victor et al., 2014; Cosgrove et al., 2014). Other potential causes include metabolic disruptions, such as hyperphosphatemia, which can promote senescence in myoblasts by impairing autophagic mechanisms, and miRNAs, which have been implicated in aging muscle and shown to alter senescent gene expression (Sosa et al., 2018; Soriano‐Arroquia et al., 2021; Hu et al., 2014).

4.1.2 Evidence against senescent cell accumulation

Unfortunately, the literature contains many conflicting reports regarding the accumulation of senescent cells in aging skeletal muscle. Several studies by the Peterson laboratory have found no difference in senescence markers between young and old skeletal muscle in both mice and humans (Dungan et al., 2021; Dungan et al., 2020; Dungan et al., 2022). These observations were confirmed by other groups who detected a very low abundance of SA-β-gal–positive cells in old muscle (Moiseeva et al., 2023; Lai et al., 2024). Furthermore, human muscle precursor cells isolated from young and old donors have been found to have negligible differences in their senescent profile (Alsharidah et al., 2013); some research has even shown that MuSCs have no change in p16 expression with aging (Zhang X. et al., 2022; Baker et al., 2013). Taken together, these observations suggest that senescent cells do not accumulate in aging skeletal muscle, in contrast to the work discussed earlier.

There are some potential explanations for the discrepancy in senescent cell accumulation within aged muscle. One theory is that the expression of these common senescence biomarkers is incredibly low. Skeletal muscle inherently has very low quantifiable γH2AX, p16, and p21 expression, while SA-β-gal staining was very rare in both young and old resting muscles (Dungan et al., 2020; Dungan et al., 2022; Moiseeva et al., 2023; Lai et al., 2024; Wang et al., 2009). The low expression of senescent biomarkers can make it challenging to accurately quantify cellular senescence and lead to differential results between studies, especially since a significant proportion of the literature utilizes a single marker, which is not the preferred approach (Gorgoulis et al., 2019). When multiple senescence markers are used instead, several studies have identified an accumulation of senescent cells in aging skeletal muscle (Zhang et al., 2022a; Da Silva et al., 2019). However, this is not always the case, as the combined use of SA-β-gal and p21 failed to detect an elevation in aged mouse muscle (Dungan et al., 2022). It is possible that this observation was affected by the fact that p21 is highly upregulated during MuSC myogenesis and thus may not be ideal for quantifying senescence in skeletal muscle (Hawke et al., 2003). Another potential explanation for the conflicting observations in aged skeletal muscle is related to the definition of “old age”. In one study, “old” mice aged 20–24 months had no change in p16+ MuSCs, while “geriatric” mice aged 28–32 months showed an increase (Sousa-Victor et al., 2014). This could also explain why some human research in adults aged 75 ± 3 found no change in senescence accumulation compared to young individuals, while other studies looking at older adults aged 83 ± 7 observed a change (García-Prat et al., 2016b; Dungan et al., 2020). Lastly, a recent review suggested that other factors, such as animal facility location, sex, fibre type composition, or spatial location of the senescent cells might also account for these discrepancies in aged skeletal muscle (Dungan et al., 2023). Emerging technologies, such as spatial transcriptomics, may soon help overcome some of the challenges with senescence characterization (such as multi-marker labelling) and reveal a more definitive picture of senescent cell accumulation with aging.

4.2 Senescent features within post-mitotic structures

Traditionally, senescence is thought to occur exclusively in mitotically capable cells, but there is a growing body of evidence suggesting that post-mitotic senescence could be possible (Sapieha and Mallette, 2018; Von Zglinicki et al., 2021). Several terminally differentiated cells have been found to accumulate multiple senescence markers with aging, including neurons, cardiomyocytes, cochlear cells and osteocytes (Jurk et al., 2012; Anderson et al., 2019; Farr et al., 2016; Benkafadar et al., 2019). The vast majority of skeletal muscle is composed of terminally differentiated myofibres and post-mitotic myonuclei, so the implication of senescence in these structures is quite significant. Human RNA-seq data from the Genotype-Tissue Expression (GTEx) project showed that p16 expression is significantly elevated in multiple tissues, including skeletal muscle (Hudgins et al., 2018). This has since been confirmed directly through RT-PCR, with old male individuals exhibiting 2- to 5-fold greater p21 and p16 mRNA expression in skeletal muscle biopsies relative to young males (Balan et al., 2020). Meanwhile, numerous studies have found that aged mice have elevated levels of p53, p21, and p16 in myofibres compared to young mice (Zhang X. et al., 2022; Sosa et al., 2018; da Silva et al., 2019; Solovyeva et al., 2021). These myofibres also have increased expression of pro-inflammatory SASP genes, including IL-1α, Il-1β, IL-6, and TNF-α (Da Silva et al., 2019). Alternatively, conflicting reports show decreased p21 protein in aged human skeletal muscle and the absence of elevated p16 mRNA in mature myofibres from BubR1 progeroid mice (Baker et al., 2013; Dethlefsen et al., 2018). Taken together, these observations indicate the potential that aged myofibres and/or their myonuclei could experience a molecular signature indicative of senescence.

The notion that post-mitotic myonuclei might be senescent is exciting. Previous work has identified senescent nuclei in aged skeletal muscle, but unfortunately, many of these studies did not utilize additional biomarkers to determine the source of these cells (Dungan et al., 2023). Myonuclei are capable of accumulating DNA damage when metabolically stressed, such as during obesity (Dungan et al., 2020). Expanding on this leads us to theorize that myonuclei could undergo mitotically-independent senescence by activating the DDR. Notably, two independent single-nuclei RNA-seq-based studies identified subpopulations of myonuclei that have elevated p21 gene expression exclusively in aged muscle samples (Zhang X. et al., 2022; Perez et al., 2022). Moreover, the myofibres of old mice contain more p21-positive myonuclei with higher levels of telomere-associated DNA damage foci (TAF), suggesting the presence of senescence in these nuclei (Da Silva et al., 2019). These observations are nicely complimented by recent evidence showing that mouse myonuclei are capable of synthesizing DNA and endoreplication (Borowik et al., 2022). These results indicate that at least a portion of myonuclei might not be post-mitotic and could experience a senescence-like phenotype. The induction of senescence within aged myofibres and/or myonuclei could have substantial effects on skeletal muscle homeostasis.

4.3 Systemic SASP cross-tissue effects on skeletal muscle

Lastly, there is a strong potential for systemic SASP factors to contribute to the altered physiology of aged skeletal muscle. The SASP, as discussed above, is an impactful characteristic of senescent cells that can exert an effect on both the cellular microenvironment and distant tissues (Coppé et al., 2010). In acute exposure, SASP factors are essential for homeostatic processes like wound healing and tumour suppression, however, chronic SASP production is associated with several detriments to tissue health (Coppé et al., 2010; Birch and Gil, 2020). The SASP factor CCL17 contributes to multi-organ fibrosis in the heart, aorta, and vascular endothelium (Zhang et al., 2023; Zhang Y. et al., 2022). Additionally, hepatocellular senescence can induce multi-tissue senescence and dysfunction through TGF-β signalling pathways, which can be reversed with senolytics that selectively eliminate senescent hepatocytes, highlighting the potential for systemic SASP effects originating from a single senescent cell type (Du et al., 2025; Kiourtis et al., 2024). During aging, we typically observe numerous adverse changes within skeletal muscle, including excessive inflammation, ECM remodelling, increased fibrosis, and altered intercellular communication–all of which are commonly associated with chronic SASP exposure (Englund et al., 2021; He et al., 2021). While it seems reasonable that the SASP of other tissues is, at least partially, contributing to these perturbations, this is an area of research that needs substantially more investigation.

The SASP signature is a moving target–various factors, such as cell type and means of senescence induction, can influence the factors that are secreted. Its composition has even been noted to change over a cell’s progression through senescence (Coppé et al., 2010; Wiley et al., 2017; Basisty et al., 2020). This makes it difficult to identify key SASP molecules or proteins that elicit their effects on skeletal muscle health and homeostasis during aging. However, certain SASP components appear to be consistent across tissues and species with high fidelity, and importantly, several of these factors are known to mediate skeletal muscle adaptations (Saul et al., 2022).

4.3.1 Pro-inflammatory SASP factors

Perhaps the most prominent and well-characterized aspect of the SASP is the pro-inflammatory factors. Given that inflammation is considered a key hallmark of aging muscle, it follows that the SASP could be a potential cause of the observed chronic inflammatory state (Coppé et al., 2010; Franceschi et al., 2018). Several studies have identified elevated levels of inflammation-related SASP factors within aged muscle (Zhang et al., 2022a; Da Silva et al., 2019; Moiseeva et al., 2023). In line with this, elevated mRNA expression of inflammatory proteins IL-1α, IL-1β, IL-6, and TNF-α have been detected within the skeletal muscle of geriatric mice (32-month-old), which was accompanied by decreases in fibre size, increases in centrally located nuclei, and greater expression of senescence markers (da Silva et al., 2019). It is also likely that circulating pro-inflammatory SASP factors originating from other tissues contribute to the chronic inflammatory state of aged muscle. Some of the strongest evidence for this comes from senescent cell transplantation experiments. Xu et al. (2018) used luciferase-expressing senescent preadipocytes with a SASP profile resembling endogenously aged senescent cells, such as the cytokines IL-6 and TNF-α, and injected them intraperitoneally into young mice (Xu et al., 2018). Two months later, luciferase-negative senescent cells and biomarkers were observed in multiple tissues, including the quadriceps muscles, indicating the recipient’s own cells underwent cellular senescence in response to SASP signals from the transplanted adipocytes (Xu et al., 2018). SASP components IL-6 and TNF-α are of particular interest as their chronically elevated expression with age is associated with several phenotypes, such as greater muscle wasting and protein catabolism, and reductions in protein synthesis rates, muscle mass and strength (Reid and Li, 2001; Schaap et al., 2006; Visser et al., 2002). This presents a plausible role for key pro-inflammatory SASP molecules like IL-6 and TNF-α in the functional decline of muscle in aging.

On a cellular level, inflammatory SASP factors have been shown to significantly impact MuSC dynamics. The transplantation of induced senescent cells into skeletal muscle resulted in DNA damage in endogenous MuSCs and increased immune cell recruitment, fibrosis, and delayed regeneration (Moiseeva et al., 2023). Moreover, TNF-α is known to impair myoblast differentiation in culture, disrupt MuSC regenerative capacity, and influence muscle atrophy through NF-κB-mediated signalling (Reid and Li, 2001; Guttridge et al., 2000; Layne and Farmer, 1999). It is also possible that inflammatory SASP components can interact with the MuSC niche, potentially dysregulating stem cell activity. Factors such as TGF-β, which promote ECM deposition, could thicken the basal lamina and impair MuSC communicative abilities (Gopinath and Rando, 2008; Ismaeel et al., 2019). Importantly, the myocytes and MuSCs of aged mice have elevated TGF-β levels that are associated with the blunted regenerative capacity of aged MuSCs (Carlson et al., 2008). Thus, there is evidence to suggest that SASP inflammatory components can interact with MuSCs through paracrine signalling, potentially disrupting them enough to contribute to their observed dysfunction with age.

4.3.2 Senescence-associated metabolites

An emerging area of research has identified that there are metabolites, such as bioactive lipids and amino acids, that are important proponents of the SASP. Preliminary investigations into the metabolic signature of senescence suggest a highly dynamic and heterogeneous metabolome occurs with senescence induction (Kamal et al., 2025; Lopes-Paciencia et al., 2019; Pundlik et al., 2024). This seems reasonable, given that a major process like cell cycle arrest is likely to influence cellular metabolism. Indeed, oncogene-activated senescent fibroblasts have elevated β-oxidation and fatty-acid breakdown (Quijano et al., 2012). Certain metabolites have been shown to modulate recipient cells in a SASP-like manner, but it is evident that others do not elicit any paracrine effects on the cellular microenvironment (Kamal et al., 2025; Lopes-Paciencia et al., 2019; Pundlik et al., 2024). Among the bioactive metabolites, lipids have garnered the most evidence as key SASP members within skeletal muscle. Some fatty acids, like arachidonic acid and oleic acid, are found at elevated concentrations within senescent cells and in their extracellular environment (Kamal et al., 2025; Lopes-Paciencia et al., 2019; Pundlik et al., 2024; Harizi et al., 2008). Inhibition of arachidonic acid-derived 15d-PGJ2 from senescent myoblasts restores muscle differentiation, highlighting the potential for bioactive lipids and their products to regulate muscle homeostasis (Pundlik et al., 2024). While these data suggest that lipids may directly influence muscle properties, it is possible that they act by stimulating the production of inflammatory SASP factors. Treating healthy myoblasts with oleic acid upregulates prominent SASP genes CCL2, CXCL12, and IL-33 (Kamal et al., 2025). Moreover, lipid depletion within senescent fibroblasts drastically reduces the production of the SASP components IL-6, CXCL-1, CXCL-10, and CXCL-5 (Ogrodnik et al., 2019). While it is important to note that most of these findings were conducted using in vitro models, they still highlight the potential for metabolites to play a key role in the expression of the SASP within aging skeletal muscle.

4.3.3 Extracellular vesicles

Another SASP component emerging as a potential mediator of muscle physiology during aging are extracellular vesicles (EVs). Serum extracted from young mice and introduced to old mice has been shown to improve muscle regeneration, but these effects were lost when the blood was depleted of EVs (Sahu et al., 2021). This has also been observed in mouse and human fibroblasts, where EVs isolated from young fibroblasts ameliorated senescence in old ones by increasing their antioxidant capacity (Fafián-Labora et al., 2020). EVs have been linked to SASP regulation, primarily through their miRNA cargo, and can affect cellular processes throughout the body via autocrine and paracrine signalling (Anakor et al., 2021; Tanaka and Takahashi, 2021). They are also thought to promote immune senescence during aging through self-contained inflammatory miRNAs (Olivieri et al., 2015). These small structures are released in large quantities following DNA damage and senescence induction and have the potential to affect multiple tissues during aging, including skeletal muscle (Tanaka and Takahashi, 2021; Lehmann et al., 2008; Alfonzo et al., 2022).

In summary, the SASP likely plays a role in the dysfunction of muscle physiology during advanced age. While pro-inflammatory SASP factors, bioactive metabolites, and EVs are promising candidates for eliciting a senescent response in aged skeletal muscle, many details remain unclear. For instance, the extent to which systemic SASP factors influence muscle homeostasis is not known; the majority of these effects may originate from neighbouring muscle cells rather than other tissues. Additional studies are needed to answer these questions, and investigations into anti-SASP therapies (i.e., senomorphics) could help us better understand the implications this feature has on aging muscle.

5 Senotherapeutic strategies to counteract muscle aging

Since the accumulation of senescent cells is a hallmark of aging, our ability to target and eliminate them is crucial. The transgenic removal of senescent cells from various tissues, including the eyes, skeletal muscle, and adipose, delayed the onset of various aging-related pathologies and extended the lifespan in mice (Baker et al., 2011). Furthermore, aged p16^INK4a–null mice had larger muscle fibres and improved exercise performance relative to their non-transgenic counterparts, suggesting that the elimination of senescent cells may be a viable approach to counteract aging-related muscle perturbations (Baker et al., 2011). First introduced in 2015, senotherapeutics represent a new class of drugs that aim to reduce the impact of cellular senescence and can be classified as either senolytics or senomorphics (Zhu et al., 2015). The key difference between these two classes is that senolytics directly target and eliminate senescent cells while senomorphics aim to alleviate the effects of the SASP (Zhu et al., 2015). Senolytics primarily act by transiently disabling the senescence cell anti-apoptotic pathway (SCAP) to promote the selective elimination of senescent cells (Kirkland and Tchkonia, 2020). Alternatively, the mechanisms governing senomorphics can vary significantly based on the targeted SASP component and are not as well-studied as senolytics in the context of skeletal muscle aging.

The first major development in senolytics was the discovery that dasatinib and quercetin (D + Q) could target pro-survival pathways and promote apoptosis in senescent cells (Zhu et al., 2015). These compounds were identified through bioinformatic analyses to determine clinically approved products that could target the SCAP network (Kirkland and Tchkonia, 2020). Dasatinib was an FDA-approved chemotherapeutic that inhibited tyrosine kinase, and quercetin was a naturally occurring flavonoid found in apple peels. The combination of D + Q has been repeatedly shown to be effective at inducing apoptosis in all types of senescent cells and is arguably the most widely used senolytic (Dungan et al., 2022; Zhu et al., 2015; Alharbi et al., 2022). Soon after, other promising senolytics were identified, such as ABT263, more commonly known as Navitoclax, which acts on the pro-survival BCL2 protein family that is naturally elevated within senescent cells to protect against apoptosis (Zhu et al., 2016; Wang, 1995; Chang et al., 2016). Natural senolytic compounds like the flavonoids quercetin and fisetin inhibit the BCL2 family and certain SCAP members (Zhu et al., 2017; Yousefzadeh et al., 2018). There are currently dozens of validated and predicted senolytic compounds, but this review will focus on a handful that have been adequately investigated within skeletal muscle, namely, Navitoclax, fisetin, dasatinib and quercetin (Figure 3).

FIGURE 3

5.1 In vitro potential of senolytic drugs

Senolytic compounds are often first examined through in vitro models of senescence. Navitoclax has been shown to selectively kill senescent cells independent of cell type, senescence induction method, or species, except for human primary pre-adipocytes (Zhu et al., 2016; Chang et al., 2016). Within the context of skeletal muscle, Navitoclax can effectively clear senescent muscle progenitor cells (MPCs) isolated from naturally aged mice and improve the number of non-senescent MPCs in vitro (Chang et al., 2016). While these results are promising, there is limited evidence for Navitoclax’s effectiveness at eliminating senescent muscle cells in vivo. The flavonoid fisetin has also been shown to be an effective senolytic for muscle-derived cells from Z24^−/− progeroid mice (Liu et al., 2022a). Senescent FAPs isolated from these mice impair the proliferation and myogenic potential of co-cultured wildtype MPCs, but these effects can be reversed with acute fisetin treatment. In C₂C₁₂ mouse myoblasts, fisetin significantly attenuated H₂O₂-induced oxidative stress and DNA damage while limiting ROS generation, all of which are known senescence inducers (Park et al., 2023). Moreover, multiple studies have reported that fisetin can alleviate senescence within vascular smooth muscle cells through the PTEN-mTORC2 signalling axis (Kim et al., 2021; Kim et al., 2023a; Kim et al., 2023b). Similarly, quercetin, either independently or in combination with dasatinib, can induce apoptosis in senescent vascular smooth muscle cells (Gadecka et al., 2025; K et al., 2020). Overall, there is ample evidence that senolytic agents are highly effective at clearing senescent muscle cells in culture, and they offer reliable experimental models for investigating the underlying mechanisms of cellular senescence in muscle.

5.2 Senolytics during muscle regeneration

Aged skeletal muscle has a reduced capacity for repair and regeneration, and treatments that improve these processes could extend healthspan and quality of life in the elderly. Senolytics can have varying effects in the skeletal muscle microenvironment, especially during periods of muscle damage. There is evidence that muscle-resident cells involved in muscle repair, namely, MuSCs, FAPs, and macrophages, can be influenced by senolytic interventions. Four weeks of treatment with fisetin in adult Z24^−/− progeroid mice increased the number of MuSCs while reducing the number of FAPs and intramuscular fibrosis and ultimately improving muscle size and strength (Liu et al., 2022a). Conversely, D + Q treatment in aged mice did not affect MuSC content or intramuscular fibrosis following BaCl₂ injury (Dungan et al., 2021). In line with this, old mice provided with D + Q for 4 months displayed fewer centrally nucleated myofibres, indicating either an impairment in the MuSC response or a reduced need for muscle regeneration (Zhang X. et al., 2022; Bi et al., 2024). This discrepancy in senolytic impact on MuSCs could be due to the diversity in compound pharmacology, animal models, and injury modalities. Alternatively, the improved muscle phenotype may be driven by the influence of senolytics on other muscle-resident cell types. Seminal work by Zhang et al. found that the administration of D + Q did not attenuate age-related declines in muscle mass or myofibre CSA, but did reduce the number of centrally located fibres and improve grip strength (Zhang X. et al., 2022). However, they reported that the senescent marker p16 was only detectable in FAPs and macrophages, suggesting that these cell types, rather than MuSCs, may be more implicated in the muscle response to senolytics. In the mdx model of DMD, short-term treatment with fisetin eliminated senescent macrophages, which in turn improved MuSC function, suggesting that senolytic use can influence muscle regenerative capacity by acting on senescent immune cells (Liu et al., 2022b). Future senotherapeutic research would benefit greatly from evaluating multiple cell populations during various states of muscle damage.

5.3 Senolytic impact on aged muscle function

As research supporting a role for senescence in the development of sarcopenia has emerged, so too has an interest in the potential for senolytics to combat skeletal muscle decline with age. Zhu and colleagues (2015) were the first to examine the effects of senolytic use on skeletal muscle. 24-month-old mice were treated with a single dose of 5 mg/kg and 50 mg/kg of D + Q, respectively (Zhu et al., 2015). They found that a single dose of D + Q reduced the number of senescent cells in 24-month-old skeletal muscle, while 6 weeks of senolytic treatment also reduced frailty index and delayed gait disorders in Ercc1^-/Δ progeroid mice (Zhu et al., 2015). Later work from this group and others showed that 4 months of D + Q treatment in aged mice (20-month-old) improved several functional metrics, including walking speed, hang time, grip strength, treadmill endurance capacity, motor coordination/balance, and daily activity levels relative to aged vehicle-treated mice (Zhang X. et al., 2022; Xu et al., 2018; Dungan et al., 2021). Another study used SOD1KO mice to model a senescent phenotype by eliciting oxidative stress-induced muscle frailty and found that 7 months of D + Q treatment effectively lowered p21 mRNA expression but did not influence muscle mass, which is in line with previous reports in aged mouse muscle (Zhang X. et al., 2022; Borowik et al., 2024). Despite this, senolytic treatment did increase muscle-specific force generation and improve mitochondrial respiration in these mice (Borowik et al., 2024). Although D + Q is the most common senolytic used in aging muscle research, other drugs such as Navitoclax have also demonstrated potential. Short-term (10 days) Navitoclax treatment in irradiated male C57BL/6 mice resulted in improvements in muscle coordination and endurance capacity (Fielder et al., 2022). Interestingly, these animals had no change in muscle CSA, fibrosis, adiposity, or p21+ cell abundance, indicating that senolytic treatment must have altered muscle function through alternative mechanisms. Overall, senolytics show promise as a potential therapeutic to improve skeletal muscle function with aging, but more research is needed to elucidate their effects and mechanisms of action within in vivo models.

6 Conclusion

Emerging evidence is linking senescence to several of the perturbations that are present in aged skeletal muscle. Despite some discrepancies in the mechanisms of action, it is clear that this cellular process can regulate aging muscle dynamics, muscle function, and the activity of several muscle-resident cell populations. Recent advances in senotherapeutic research also provide novel strategies for combating or delaying aging. However, our understanding of senescence in the context of skeletal muscle is incomplete, and more work is required to fully elucidate the mechanisms governing senescent regulation of skeletal muscle.

References

• 1

  Acosta J. C. O’Loghlen A. Banito A. Guijarro M. V. Augert A. Raguz S. et al (2008). Chemokine signaling via the CXCR2 receptor reinforces senescence. Cell133 (6), 1006–1018. 10.1016/j.cell.2008.03.038

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 2

  Acosta J. C. Banito A. Wuestefeld T. Georgilis A. Janich P. Morton J. P. et al (2013). A complex secretory program orchestrated by the inflammasome controls paracrine senescence. Nat. Cell Biol.15 (8), 978–990. 10.1038/ncb2784

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 3

  Alfonzo M. C. Al Saedi A. Fulzele S. Hamrick M. W. (2022). Extracellular vesicles as communicators of senescence in musculoskeletal aging. JBMR Plus6 (11), e10686. 10.1002/jbm4.10686

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 4

  Alharbi K. S. Afzal O. Altamimi A. S. A. Almalki W. H. Kazmi I. Al-Abbasi F. A. et al (2022). A study of the molecular mechanism of quercetin and dasatinib combination as senolytic in alleviating age-related and kidney diseases. J. Food Biochem.46 (12), e14471. 10.1111/jfbc.14471

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 5

  Alsharidah M. Lazarus N. R. George T. E. Agley C. C. Velloso C. P. Harridge S. D. R. (2013). Primary human muscle precursor cells obtained from young and old donors produce similar proliferative, differentiation and senescent profiles in culture. Aging Cell12 (3), 333–344. 10.1111/acel.12051

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 6

  Anakor E. Le Gall L. Dumonceaux J. Duddy W. J. Duguez S. (2021). Exosomes in ageing and motor neurone disease: biogenesis, uptake mechanisms, modifications in disease and uses in the development of biomarkers and therapeutics. Cells10 (11), 2930. 10.3390/cells10112930

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 7

  Ancel S. Stuelsatz P. Feige J. N. (2021). Muscle stem cell quiescence: controlling stemness by staying asleep. Trends Cell Biol.31 (7), 556–568. 10.1016/j.tcb.2021.02.006

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 8

  Anderson R. Lagnado A. Maggiorani D. Walaszczyk A. Dookun E. Chapman J. et al (2019). Length‐independent telomere damage drives post‐mitotic cardiomyocyte senescence. EMBO J.38 (5), e100492. 10.15252/EMBJ.2018100492

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 9

  Asakura A. Komaki M. Rudnicki M. A. (2001). Muscle satellite cells are multipotential stem cells that exhibit myogenic, osteogenic, and adipogenic differentiation. Differ. Res. Biol. Divers68 (4–5), 245–253. 10.1046/j.1432-0436.2001.680412.x

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 10

  Baker D. J. Perez-Terzic C. Jin F. Pitel K. S. Niederländer N. J. Jeganathan K. et al (2008). Opposing roles for p16Ink4a and p19Arf in senescence and ageing caused by BubR1 insufficiency. Nat. Cell Biol.10 (7), 825–836. 10.1038/ncb1744

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 11

  Baker D. J. Wijshake T. Tchkonia T. LeBrasseur N. K. Childs B. G. van de Sluis B. et al (2011). Clearance of p16Ink4a-positive senescent cells delays ageing-associated disorders. Nature479 (7372), 232–236. 10.1038/nature10600

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 12

  Baker D. J. Weaver R. L. van Deursen J. M. (2013). p21 both attenuates and drives senescence and aging in BubR1 progeroid mice. Cell Rep.3 (4), 1164–1174. 10.1016/j.celrep.2013.03.028

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 13

  Baker D. J. Childs B. G. Durik M. Wijers M. E. Sieben C. J. Zhong J. et al (2016). Naturally occurring p16 Ink4a-positive cells shorten healthy lifespan. Nature530 (7589), 184–189. 10.1038/nature16932

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 14

  Balan E. de Groote E. Bouillon M. Viceconte N. Mahieu M. Naslain D. et al (2020). No effect of the endurance training status on senescence despite reduced inflammation in skeletal muscle of older individuals. Am. J. Physiol. - Endocrinol. Metab.319 (2), E447–E454. 10.1152/ajpendo.00149.2020

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 15

  Basisty N. Kale A. Jeon O. H. Kuehnemann C. Payne T. Rao C. et al (2020). A proteomic atlas of senescence-associated secretomes for aging biomarker development. PLOS Biol.18 (1), e3000599. 10.1371/journal.pbio.3000599

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 16

  Benkafadar N. François F. Affortit C. Casas F. Ceccato J. C. Menardo J. et al (2019). ROS-induced activation of DNA damage responses drives senescence-like state in postmitotic cochlear cells: implication for hearing preservation. Mol. Neurobiol.56 (8), 5950–5969. 10.1007/s12035-019-1493-6

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 17

  Bi W. Yang M. Shi M. Hou M. Jiang C. Fan G. et al (2024). A comprehensive single-cell RNA transcriptomic analysis identifies a unique SPP1+ macrophages subgroup in aging skeletal muscle. Sci. Rep.14 (1), 18156. 10.1038/s41598-024-69284-9

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 18

  Birch J. Gil J. (2020). Senescence and the SASP: many therapeutic avenues. Genes Dev.34 (23–24), 1565–1576. 10.1101/gad.343129.120

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 19

  Bodnar A. G. Ouellette M. Frolkis M. Holt S. E. Chiu C. P. Morin G. B. et al (1998). Extension of life-span by introduction of telomerase into normal human cells. Science279 (5349), 349–352. 10.1126/science.279.5349.349

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 20

  Borowik A. K. Davidyan A. Peelor F. F. Voloviceva E. Doidge S. M. Bubak M. P. et al (2022). Skeletal muscle nuclei in mice are not post-mitotic. Function4 (1), zqac059. 10.1093/function/zqac059

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 21

  Borowik A. K. Lawrence M. M. Peelor F. F. Piekarz K. M. Crosswhite A. Richardson A. et al (2024). Senolytic treatment does not mitigate oxidative stress-induced muscle atrophy but improves muscle force generation in CuZn superoxide dismutase knockout mice. GeroScience46 (3), 3219–3233. 10.1007/s11357-024-01070-x

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 22

  Brett J. O. Arjona M. Ikeda M. Quarta M. de Morrée A. Egner I. M. et al (2020). Exercise rejuvenates quiescent skeletal muscle stem cells in old mice through restoration of cyclin D1. Nat. Metab.2 (4), 307–317. 10.1038/s42255-020-0190-0

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 23

  Buj R. Leon K. E. Anguelov M. A. Aird K. M. (2021). Suppression of p16 alleviates the senescence-associated secretory phenotype. Aging13 (3), 3290–3312. 10.18632/aging.202640

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 24

  Campisi J. (1997). The biology of replicative senescence. Eur. J. Cancer33 (5), 703–709. 10.1016/S0959-8049(96)00058-5

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 25

  Campisi J. D’Adda Di Fagagna F. (2007). Cellular senescence: when bad things happen to good cells. Nat. Rev. Mol. Cell Biol.8 (9), 729–740. 10.1038/nrm2233

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 26

  Carlson M. E. Hsu M. Conboy I. M. (2008). Imbalance between pSmad3 and notch induces CDK inhibitors in old muscle stem cells. Nature454 (7203), 528–532. 10.1038/nature07034

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 27

  Chakkalakal J. V. Jones K. M. Basson M. A. Brack A. S. (2012). The aged niche disrupts muscle stem cell quiescence. Nature490 (7420), 355–360. 10.1038/nature11438

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 28

  Chandeck C. Mooi W. J. (2010). Oncogene-induced cellular senescence. Adv. Anat. Pathol.17 (1), 42–48. 10.1097/PAP.0b013e3181c66f4e

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 29

  Chang J. Wang Y. Shao L. Laberge R. M. Demaria M. Campisi J. et al (2016). Clearance of senescent cells by ABT263 rejuvenates aged hematopoietic stem cells in mice. Nat. Med.22 (1), 78–83. 10.1038/nm.4010

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 30

  Chen X. Li Z. Feng Z. Wang J. Ouyang C. Liu W. et al (2006). Integrin-linked kinase induces both senescence-associated alterations and extracellular fibronectin assembly in aging cardiac fibroblasts. J. Gerontol. Ser. A61 (12), 1232–1245. 10.1093/gerona/61.12.1232

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 31

  Chicas A. Wang X. Zhang C. McCurrach M. Zhao Z. Mert O. et al (2010). Dissecting the unique role of the retinoblastoma tumor suppressor during cellular senescence. Cancer Cell17 (4), 376–387. 10.1016/j.ccr.2010.01.023

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 32

  Chien Y. Scuoppo C. Wang X. Fang X. Balgley B. Bolden J. E. et al (2011). Control of the senescence-associated secretory phenotype by NF-κB promotes senescence and enhances chemosensitivity. Genes Dev.25 (20), 2125–2136. 10.1101/gad.17276711

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 33

  Cho K. A. Ryu S. J. Oh Y. S. Park J. H. Lee J. W. Kim H. P. et al (2004). Morphological adjustment of senescent cells by modulating caveolin-1 status. J. Biol. Chem.279 (40), 42270–42278. 10.1074/jbc.M402352200

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 34

  Chrétien A. Piront N. Delaive E. Demazy C. Ninane N. Toussaint O. (2008). Increased abundance of cytoplasmic and nuclear caveolin 1 in human diploid fibroblasts in H₂O₂‐induced premature senescence and interplay with p38α^MAPK. FEBS Lett.582 (12), 1685–1692. 10.1016/j.febslet.2008.04.026

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 35

  Conboy I. M. Conboy M. J. Wagers A. J. Girma E. R. Weissman I. L. Rando T. A. (2005). Rejuvenation of aged progenitor cells by exposure to a young systemic environment. Nature433 (7027), 760–764. 10.1038/nature03260

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 36

  Collado M. Blasco M. A. Serrano M. (2007). Cellular senescence in cancer and aging. Cell130 (2), 223–233. 10.1016/j.cell.2007.07.003

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 37

  Conboy I. M. Rando T. A. (2005). Aging, stem cells and tissue regeneration: lessons from muscle. Cell Cycle4 (3), 407–410. 10.4161/cc.4.3.1518

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 38

  Coppé J. P. Patil C. K. Rodier F. Sun Y. Muñoz D. P. Goldstein J. et al (2008). Senescence-associated secretory phenotypes reveal cell-nonautonomous functions of oncogenic RAS and the p53 tumor suppressor. PLOS Biol.6 (12), 2853–2868. 10.1371/journal.pbio.0060301

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 39

  Coppé J. P. Desprez P. Y. Krtolica A. Campisi J. (2010). The senescence-associated secretory phenotype: the dark side of tumor suppression. Annu. Rev. Pathol. Mech. Dis.5 (1), 99–118. 10.1146/annurev-pathol-121808-102144

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 40

  Cosgrove B. D. Gilbert P. M. Porpiglia E. Mourkioti F. Lee S. P. Corbel S. Y. et al (2014). Rejuvenation of the muscle stem cell population restores strength to injured aged muscles. Nat. Med.20 (3), 255–264. 10.1038/nm.3464

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 41

  Cruz-Jentoft A. J. Sayer A. A. (2019). Sarcopenia. Lancet393 (10191), 2636–2646. 10.1016/S0140-6736(19)31138-9

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 42

  da Silva P. F. L. Ogrodnik M. Kucheryavenko O. Glibert J. Miwa S. Cameron K. et al (2019). The bystander effect contributes to the accumulation of senescent cells in vivo. Aging Cell18 (1), e12848. 10.1111/acel.12848

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 43

  Dasari A. Bartholomew J. N. Volonte D. Galbiati F. (2006). Oxidative stress induces premature senescence by stimulating caveolin-1 gene transcription through p38 mitogen-activated protein kinase/Sp1-mediated activation of two GC-rich promoter elements. Cancer Res.66 (22), 10805–10814. 10.1158/0008-5472.CAN-06-1236

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 44

  Demaria M. Ohtani N. Youssef S. A. Rodier F. Toussaint W. Mitchell J. R. et al (2014). An essential role for senescent cells in optimal wound healing through secretion of PDGF-AA. Dev. Cell31 (6), 722–733. 10.1016/j.devcel.2014.11.012

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 45

  Dethlefsen M. M. Halling J. F. Møller H. D. Plomgaard P. Regenberg B. Ringholm S. et al (2018). Regulation of apoptosis and autophagy in mouse and human skeletal muscle with aging and lifelong exercise training. Exp. Gerontol.111 (July), 141–153. 10.1016/j.exger.2018.07.011

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 46

  Dimri G. P. Lee X. Basile G. Acosta M. Scott G. Roskelley C. et al (1995). A biomarker that identifies senescent human cells in culture and in aging skin in vivo. Proc. Natl. Acad. Sci. U. S. A.92 (20), 9363–9367. 10.1073/pnas.92.20.9363

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 47

  Disayabutr S. Kim E. K. Cha S. I. Green G. Naikawadi R. P. Jones K. D. et al (2016). miR-34 miRNAs regulate cellular senescence in type II alveolar epithelial cells of patients with idiopathic pulmonary fibrosis. PLOS ONE11 (6), e0158367. 10.1371/journal.pone.0158367

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 48

  Du K. Umbaugh D. S. Wang L. Jun J. H. Dutta R. K. Oh S. H. et al (2025). Targeting senescent hepatocytes for treatment of metabolic dysfunction-associated steatotic liver disease and multi-organ dysfunction. Nat. Commun.16 (1), 3038. 10.1038/s41467-025-57616-w

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 49

  Dungan C. M. Peck B. D. Walton R. G. Huang Z. Bamman M. M. Kern P. A. et al (2020). In vivo analysis of γH2AX+ cells in skeletal muscle from aged and Obese humans. FASEB J.34 (5), 7018–7035. 10.1096/fj.202000111RR

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 50

  Dungan C. M. Murach K. A. Zdunek C. J. Tang Z. J. VonLehmden G. L. Brightwell C. R. et al (2021). Deletion of SA β‐Gal+ cells using senolytics improves muscle regeneration in old mice. Aging Cell21, e13528–17. 10.1111/acel.13528

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 51

  Dungan C. M. Figueiredo V. C. Wen Y. VonLehmden G. L. Zdunek C. J. Thomas N. T. et al (2022). Senolytic treatment rescues blunted muscle hypertrophy in old mice. GeroScience44 (4), 1925–1940. 10.1007/s11357-022-00542-2

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 52

  Dungan C. M. Wells J. M. Murach K. A. (2023). The life and times of cellular senescence in skeletal muscle: friend or foe for homeostasis and adaptation?Am. J. Physiol-Cell Physiol.325 (1), C324–C331. 10.1152/ajpcell.00553.2022

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 53

  d’Adda di Fagagna F. Reaper P. M. Clay-Farrace L. Fiegler H. Carr P. von Zglinicki T. et al (2003). A DNA damage checkpoint response in telomere-initiated senescence. Nature426 (6963), 194–198. 10.1038/nature02118

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 54

  Englund D. A. Murach K. A. Dungan C. M. Figueiredo V. C. Vechetti I. J. Dupont-Versteegden E. E. et al (2020). Depletion of resident muscle stem cells negatively impacts running volume, physical function, and muscle fiber hypertrophy in response to lifelong physical activity. Am. J. Physiol. - Cell Physiol.318 (6), C1178–C1188. 10.1152/ajpcell.00090.2020

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 55

  Englund D. A. Zhang X. Aversa Z. LeBrasseur N. K. (2021). Skeletal muscle aging, cellular senescence, and senotherapeutics: current knowledge and future directions. Mech. Ageing Dev.200 (August), 111595. 10.1016/j.mad.2021.111595

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 56

  Evano B. Gill D. Hernando-Herraez I. Comai G. Stubbs T. M. Commere P. H. et al (2020). Transcriptome and epigenome diversity and plasticity of muscle stem cells following transplantation. PLOS Genet.16 (10), e1009022. 10.1371/journal.pgen.1009022

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 57

  Fabian M. R. Sonenberg N. Filipowicz W. (2010). Regulation of mRNA translation and stability by microRNAs. Annu. Rev. Biochem.79 (79), 351–379. 10.1146/annurev-biochem-060308-103103

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 58

  Fafián-Labora J. A. Rodríguez-Navarro J. A. O’Loghlen A. (2020). Small extracellular vesicles have GST activity and ameliorate senescence-related tissue damage. Cell Metab.32 (1), 71–86.e5. 10.1016/j.cmet.2020.06.004

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 59

  Faget D. V. Ren Q. Stewart S. A. (2019). Unmasking senescence: context-dependent effects of SASP in cancer. Nat. Rev. Cancer19 (8), 439–453. 10.1038/s41568-019-0156-2

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 60

  Farr J. N. Fraser D. G. Wang H. Jaehn K. Ogrodnik M. B. Weivoda M. M. et al (2016). Identification of senescent cells in the bone microenvironment. J. Bone Min. Res. Off. J. Am. Soc. Bone Min. Res.31 (11), 1920–1929. 10.1002/jbmr.2892

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 61

  Fielder E. Wan T. Alimohammadiha G. Ishaq A. Low E. Weigand B. M. et al (2022). “Short senolytic or senostatic interventions rescue progression of radiation-induced frailty and premature ageing in mice,”eLife. Editor IsalesC.11e75492. 10.7554/eLife.75492

  • CrossRef
  • Google Scholar

• 62

  Formicola L. Marazzi G. Sassoon D. A. (2014). The extraocular muscle stem cell niche is resistant to ageing and disease. Front. Aging Neurosci.6 (DEC), 328. 10.3389/fnagi.2014.00328

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 63

  Freund A. Patil C. K. Campisi J. (2011). p38MAPK is a novel DNA damage response‐independent regulator of the senescence‐associated secretory phenotype. EMBO J.30 (8), 1536–1548. 10.1038/emboj.2011.69

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 64

  Franceschi C. Garagnani P. Parini P. Giuliani C. Santoro A. (2018). Inflammaging: a new immune-metabolic viewpoint for age-related diseases. Nat. Rev. Endocrinol.14 (10), 576–590. 10.1038/s41574-018-0059-4

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 65

  Freund A. Laberge R. M. Demaria M. Campisi J. (2012). Lamin B1 loss is a senescence-associated biomarker. Mol. Biol. Cell23 (11), 2066–2075. 10.1091/mbc.E11-10-0884

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 66

  Fry C. S. Lee J. D. Mula J. Kirby T. J. Jackson J. R. Liu F. et al (2015). Inducible depletion of satellite cells in adult, sedentary mice impairs muscle regenerative capacity without affecting sarcopenia. Nat. Med.21 (1), 76–80. 10.1038/nm.3710

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 67

  Fulle S. Sancilio S. Mancinelli R. Gatta V. Di Pietro R. (2013). Dual role of the caspase enzymes in satellite cells from aged and young subjects. Cell Death Dis.4 (12), e955. 10.1038/cddis.2013.472

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 68

  Fumagalli M. Rossiello F. Clerici M. Barozzi S. Cittaro D. Kaplunov J. M. et al (2012). Telomeric DNA damage is irreparable and causes persistent DNA-damage-response activation. Nat. Cell Biol.14 (4), 355–365. 10.1038/ncb2466

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 69

  Gadecka A. Nowak N. Bulanda E. Janiszewska D. Dudkowska M. Sikora E. et al (2025). The senolytic cocktail, dasatinib and quercetin, impacts the chromatin structure of both young and senescent vascular smooth muscle cells. GeroScience47 (3), 3907–3925. 10.1007/s11357-024-01504-6

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 70

  García-Prat L. Muñoz-Cánoves P. Martinez-Vicente M. (2016a). Dysfunctional autophagy is a driver of muscle stem cell functional decline with aging. Autophagy12 (3), 612–613. 10.1080/15548627.2016.1143211

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 71

  García-Prat L. Martínez-Vicente M. Perdiguero E. Ortet L. Rodríguez-Ubreva J. Rebollo E. et al (2016b). Autophagy maintains stemness by preventing senescence. Nature529 (7584), 37–42. 10.1038/nature16187

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 72

  García-Prat L. Perdiguero E. Alonso-Martín S. Dell’Orso S. Ravichandran S. Brooks S. R. et al (2020). FoxO maintains a genuine muscle stem-cell quiescent state until geriatric age. Nat. Cell Biol.22 (11), 1307–1318. 10.1038/s41556-020-00593-7

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 73

  Gire V. Dulić V. (2015). Senescence from G2 arrest, revisited. Cell Cycle14 (3), 297–304. 10.1080/15384101.2014.1000134

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 74

  Gopinath S. D. Rando T. A. (2008). Stem cell review series: aging of the skeletal muscle stem cell niche. Aging Cell7 (4), 590–598. 10.1111/j.1474-9726.2008.00399.x

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 75

  Gorgoulis V. Adams P. D. Alimonti A. Bennett D. C. Bischof O. Bishop C. et al (2019). Cellular senescence: defining a path forward. Cell179 (4), 813–827. 10.1016/j.cell.2019.10.005

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 76

  Granic A. Suetterlin K. Shavlakadze T. Grounds M. D. Sayer A. A. (2023). Hallmarks of ageing in human skeletal muscle and implications for understanding the pathophysiology of sarcopenia in women and men. Clin. Sci.137 (22), 1721–1751. 10.1042/CS20230319

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 77

  Guttridge D. C. Mayo M. W. Madrid L. V. Wang C. Y. Baldwin A. S. (2000). NF-kappaB-induced loss of MyoD messenger RNA: possible role in muscle decay and cachexia. Sci. 2000 Sept29 (5488), 2363–2366. 10.1126/science.289.5488.2363

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 78

  Guzman S. D. Judge J. Shigdar S. M. Paul T. A. Davis C. S. Macpherson P. C. et al (2022). Removal of p16INK4 expressing cells in late life has moderate beneficial effects on skeletal muscle function in Male mice. Front. Aging2, 821904. 10.3389/fragi.2021.821904

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 79

  Harrison R. G. Greenman M. J. Mall F. P. Jackson C. M. (1907). Observations of the living developing nerve fiber. Anat. Rec.1 (5), 116–128. 10.1002/ar.1090010503

  • CrossRef
  • Google Scholar

• 80

  Hara H. Araya J. Ito S. Kobayashi K. Takasaka N. Yoshii Y. et al (2013). Mitochondrial fragmentation in cigarette smoke-induced bronchial epithelial cell senescence. Am. J. Physiol. Lung Cell Mol. Physiol.305 (10), L737–L746. 10.1152/ajplung.00146.2013

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 81

  Harizi H. Corcuff J. B. Gualde N. (2008). Arachidonic-acid-derived eicosanoids: roles in biology and immunopathology. Trends Mol. Med.14 (10), 461–469. 10.1016/j.molmed.2008.08.005

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 82

  Hawke T. J. Meeson A. P. Jiang N. Graham S. Hutcheson K. DiMaio J. M. et al (2003). p21 is essential for normal myogenic progenitor cell function in regenerating skeletal muscle. Am. J. Physiol-Cell Physiol.285 (5), C1019–C1027. 10.1152/ajpcell.00055.2003

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 83

  Hayflick L. Moorhead P. S. (1961). The serial cultivation of human diploid cell strains. Exp. Cell Res.25 (3), 585–621. 10.1016/0014-4827(61)90192-6

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 84

  He Y. Xie W. Li H. Jin H. Zhang Y. Li Y. (2021). Cellular senescence in sarcopenia: possible mechanisms and therapeutic potential. Front. Cell Dev. Biol.9, 793088. 10.3389/fcell.2021.793088

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 85

  Hernandez-Segura A. De Jong T. V. Melov S. Guryev V. Campisi J. Demaria M. (2017). Unmasking transcriptional heterogeneity in senescent cells. Curr. Biol.27 (17), 2652–2660.e4. 10.1016/j.cub.2017.07.033

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 86

  Herranz N. Gallage S. Mellone M. Wuestefeld T. Klotz S. Hanley C. J. et al (2015). mTOR regulates MAPKAPK2 translation to control the senescence-associated secretory phenotype. Nat. Cell Biol.17 (9), 1205–1217. 10.1038/ncb3225

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 87

  Hoare M. Ito Y. Kang T. W. Weekes M. P. Matheson N. J. Patten D. A. et al (2016). NOTCH1 mediates a switch between two distinct secretomes during senescence. Nat. Cell Biol.18 (9), 979–992. 10.1038/ncb3397

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 88

  Höhn A. Weber D. Jung T. Ott C. Hugo M. Kochlik B. et al (2017). Happily (n)ever after: aging in the context of oxidative stress, proteostasis loss and cellular senescence. Redox Biol.11, 482–501. 10.1016/j.redox.2016.12.001

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 89

  Hong X. Isern J. Campanario S. Perdiguero E. Ramírez-Pardo I. Segalés J. et al (2022). Mitochondrial dynamics maintain muscle stem cell regenerative competence throughout adult life by regulating metabolism and mitophagy. Cell Stem Cell29 (9), 1506–1508. 10.1016/j.stem.2022.09.002

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 90

  Hu Z. Klein J. D. Mitch W. E. Zhang L. Martinez I. Wang X. H. (2014). MicroRNA-29 induces cellular senescence in aging muscle through multiple signaling pathways. Aging6 (3), 160–175. 10.18632/aging.100643

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 91

  Huang W. Hickson L. J. Eirin A. Kirkland J. L. Lerman L. O. (2022). Cellular senescence: the good, the bad and the unknown. Nat. Rev. Nephrol.18 (10), 611–627. 10.1038/s41581-022-00601-z

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 92

  Hudgins A. D. Tazearslan C. Tare A. Zhu Y. Huffman D. Suh Y. (2018). Age- and tissue-specific expression of senescence biomarkers in mice. Front. Genet.9 (FEB), 59–6. 10.3389/fgene.2018.00059

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 93

  Ismaeel A. Kim J. S. Kirk J. S. Smith R. S. Bohannon W. T. Koutakis P. (2019). Role of transforming growth Factor-β in skeletal muscle fibrosis: a review. Int. J. Mol. Sci.20 (10), 2446. 10.3390/ijms20102446

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 94

  James E. L. Michalek R. D. Pitiyage G. N. de Castro A. M. Vignola K. S. Jones J. et al (2015). Senescent human fibroblasts show increased glycolysis and redox homeostasis with extracellular metabolomes that overlap with those of irreparable DNA damage, aging, and disease. J. Proteome Res.14 (4), 1854–1871. 10.1021/pr501221g

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 95

  Jejurikar S. S. Henkelman E. A. Cederna P. S. Marcelo C. L. Urbanchek M. G. Kuzon W. M. (2006). Aging increases the susceptibility of skeletal muscle derived satellite cells to apoptosis. Exp. Gerontol.41 (9), 828–836. 10.1016/j.exger.2006.06.053

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 96

  Jurk D. Wang C. Miwa S. Maddick M. Korolchuk V. Tsolou A. et al (2012). Postmitotic neurons develop a p21-dependent senescence-like phenotype driven by a DNA damage response. Aging Cell11 (6), 996–1004. 10.1111/j.1474-9726.2012.00870.x

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 97

  Kim S. G. Sung J. Y. Kim J. R. Choi H. C. (2020). Quercetin-induced apoptosis ameliorates vascular smooth muscle cell senescence through AMP-Activated protein kinase signaling pathway. Korean J. Physiol. Pharmacol.24 (1), 69–79. 10.4196/kjpp.2020.24.1.69

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 98

  Kamal M. Shanmuganathan M. Kroezen Z. Joanisse S. Britz-McKibbin P. Parise G. (2025). Senescent myoblasts exhibit an altered exometabolome that is linked to senescence-associated secretory phenotype signaling. Am. J. Physiol-Cell Physiol.328 (2), C440–C451. 10.1152/ajpcell.00880.2024

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 99

  Kaminski H. J. Al‐Hakim M. Leigh R. J. Bashar M. K. Ruff R. L. (1992). Extraocular muscles are spared in advanced duchenne dystrophy. Ann. Neurol.32 (4), 586–588. 10.1002/ana.410320418

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 100

  Kang H. T. Lee K. B. Kim S. Y. Choi H. R. Park S. C. (2011). Autophagy impairment induces premature senescence in primary human fibroblasts. PloS One6 (8), e23367. 10.1371/journal.pone.0023367

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 101

  Keefe A. C. Lawson J. A. Flygare S. D. Fox Z. D. Colasanto M. P. Mathew S. J. et al (2015). Muscle stem cells contribute to myofibres in sedentary adult mice. Nat. Commun.6 (1), 7087. 10.1038/ncomms8087

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 102

  Khokhlov A. N. (2013). Evolution of the term “cellular senescence” and its impact on the current cytogerontological research. Mosc Univ. Biol. Sci. Bull.68 (4), 158–161. 10.3103/s0096392513040123

  • CrossRef
  • Google Scholar

• 103

  Kim S. G. Sung J. Y. Kim J. R. Choi H. C. (2021). Fisetin-induced PTEN expression reverses cellular senescence by inhibiting the mTORC2-Akt Ser473 phosphorylation pathway in vascular smooth muscle cells. Exp. Gerontol.156, 111598. 10.1016/j.exger.2021.111598

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 104

  Kim S. G. Sung J. Y. Kang Y. J. Choi H. C. (2023a). PPARγ activation by fisetin mitigates vascular smooth muscle cell senescence via the mTORC2-FoxO3a-autophagy signaling pathway. Biochem. Pharmacol.218, 115892. 10.1016/j.bcp.2023.115892

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 105

  Kim S. G. Sung J. Y. Kang Y. J. Choi H. C. (2023b). Fisetin alleviates cellular senescence through PTEN mediated inhibition of PKCδ-NOX1 pathway in vascular smooth muscle cells. Arch. Gerontol. Geriatr.108, 104927. 10.1016/j.archger.2023.104927

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 106

  Kimmel J. C. Hwang A. B. Scaramozza A. Marshall W. F. Brack A. S. (2020). Aging induces aberrant state transition kinetics in murine muscle stem cells. Development147 (9), dev183855. 10.1242/dev.183855

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 107

  Kiourtis C. Terradas-Terradas M. Gee L. M. May S. Georgakopoulou A. Collins A. L. et al (2024). Hepatocellular senescence induces multi-organ senescence and dysfunction via TGFβ. Nat. Cell Biol.26 (12), 2075–2083. 10.1038/s41556-024-01543-3

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 108

  Kirkland J. L. Tchkonia T. (2020). Senolytic drugs: from discovery to translation. J. Intern Med.288 (5), 518–536. 10.1111/joim.13141

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 109

  Kondoh H. Lleonart M. E. Gil J. Wang J. Degan P. Peters G. et al (2005). Glycolytic enzymes can modulate cellular life span. Cancer Res.65 (1), 177–185. 10.1158/0008-5472.177.65.1

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 110

  Korolchuk V. I. Miwa S. Carroll B. von Zglinicki T. (2017). Mitochondria in cell senescence: is mitophagy the weakest link?EBioMedicine21, 7–13. 10.1016/j.ebiom.2017.03.020

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 111

  Kuang S. Kuroda K. Le Grand F. Rudnicki M. A. (2007). Asymmetric self-renewal and commitment of satellite stem cells in muscle. Cell129 (5), 999–1010. 10.1016/j.cell.2007.03.044

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 112

  Kumari R. Jat P. (2021). Mechanisms of cellular senescence: cell cycle arrest and senescence associated secretory phenotype. Front. Cell Dev. Biol.9, 645593. 10.3389/fcell.2021.645593

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 113

  Lai Y. Ramírez-Pardo I. Isern J. An J. Perdiguero E. Serrano A. L. et al (2024). Multimodal cell atlas of the ageing human skeletal muscle. Nature629 (8010), 154–164. 10.1038/s41586-024-07348-6

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 114

  Layne M. D. Farmer S. R. (1999). Tumor necrosis Factor-α and basic fibroblast growth factor differentially inhibit the insulin-like growth Factor-I induced expression of myogenin in C2C12 myoblasts. Exp. Cell Res.249 (1), 177–187. 10.1006/excr.1999.4465

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 115

  Lee A. H. Ghosh D. Koh I. L. Dawson M. R. (2023). Senescence-associated exosomes transfer miRNA-induced fibrosis to neighboring cells. Aging15 (5), 1237–1256. 10.18632/aging.204539

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 116

  Lehmann B. D. Paine M. S. Brooks A. M. McCubrey J. A. Renegar R. H. Wang R. et al (2008). Senescence-associated exosome release from human prostate cancer cells. Cancer Res.68 (19), 7864–7871. 10.1158/0008-5472.CAN-07-6538

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 117

  Li J. Han S. Cousin W. Conboy I. M. (2015). Age-specific functional epigenetic changes in p21 and p16 in injury-activated satellite cells. Stem Cells33 (3), 951–961. 10.1002/stem.1908

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 118

  Li X. Li C. Zhang W. Wang Y. Qian P. Huang H. (2023). Inflammation and aging: signaling pathways and intervention therapies. Signal Transduct. Target Ther.8 (1), 239–29. 10.1038/s41392-023-01502-8

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 119

  Liu D. Hornsby P. J. (2007). Senescent human fibroblasts increase the early growth of xenograft tumors via matrix metalloproteinase secretion. Cancer Res.67 (7), 3117–3126. 10.1158/0008-5472.CAN-06-3452

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 120

  Liu L. Yue X. Sun Z. Hambright W. S. Wei J. Li Y. et al (2022a). Reduction of senescent fibro‐adipogenic progenitors in progeria‐aged muscle by senolytics rescues the function of muscle stem cells. J. Cachexia Sarcopenia Muscle13 (6), 3137–3148. 10.1002/jcsm.13101

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 121

  Liu L. Yue X. Sun Z. Hambright W. S. Feng Q. Cui Y. et al (2022b). Senolytic elimination of senescent macrophages restores muscle stem cell function in severely dystrophic muscle. Aging14 (19), 7650–7661. 10.18632/aging.204275

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 122

  Lopes-Paciencia S. Saint-Germain E. Rowell M. C. Ruiz A. F. Kalegari P. Ferbeyre G. (2019). The senescence-associated secretory phenotype and its regulation. Cytokine117, 15–22. 10.1016/j.cyto.2019.01.013

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 123

  López-Otín C. Blasco M. A. Partridge L. Serrano M. Kroemer G. (2023). Hallmarks of aging: an expanding universe. Cell.186 (2), 243–278. 10.1016/j.cell.2022.11.001

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 124

  Mabrouk N. Ghione S. Laurens V. Plenchette S. Bettaieb A. Paul C. (2020). Senescence and cancer: role of nitric oxide (NO) in SASP. Cancers12 (5), 1145. 10.3390/cancers12051145

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 125

  Mademtzoglou D. Relaix F. (2022). From cyclins to CDKIs: cell cycle regulation of skeletal muscle stem cell quiescence and activation. Exp. Cell Res.420 (1), 113275. 10.1016/j.yexcr.2022.113275

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 126

  Matsuda S. Revandkar A. Dubash T. D. Ravi A. Wittner B. S. Lin M. et al (2023). TGF-β in the microenvironment induces a physiologically occurring immune-suppressive senescent state. Cell Rep.42 (3), 112129. 10.1016/j.celrep.2023.112129

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 127

  Megeney L. A. Kablar B. Garrett K. Anderson J. E. Rudnicki M. A. (1996). MyoD is required for myogenic stem cell function in adult skeletal muscle. Genes Dev.10 (10), 1173–1183. 10.1101/gad.10.10.1173

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 128

  Miwa S. Kashyap S. Chini E. von Zglinicki T. (2022). Mitochondrial dysfunction in cell senescence and aging. J. Clin. Invest132 (13), e158447. 10.1172/JCI158447

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 129

  Moiseeva V. Cisneros A. Sica V. Deryagin O. Lai Y. Jung S. et al (2023). Senescence atlas reveals an aged-like inflamed niche that blunts muscle regeneration. Nature613 (7942), 169–178. 10.1038/s41586-022-05535-x

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 130

  Muñoz-Espín D. Serrano M. (2014). Cellular senescence: from physiology to pathology. Nat. Rev. Mol. Cell Biol.15 (7), 482–496. 10.1038/nrm3823

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 131

  Muñoz-Espín D. Cañamero M. Maraver A. Gómez-López G. Contreras J. Murillo-Cuesta S. et al (2013). Programmed cell senescence during mammalian embryonic development. Cell155 (5), 1104–1118. 10.1016/j.cell.2013.10.019

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 132

  Narzt M. S. Pils V. Kremslehner C. Nagelreiter I. M. Schosserer M. Bessonova E. et al (2021). Epilipidomics of senescent dermal fibroblasts identify lysophosphatidylcholines as pleiotropic senescence-associated secretory phenotype (SASP) factors. J. Invest Dermatol141 (4), 993–1006.e15. 10.1016/j.jid.2020.11.020

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 133

  Ogrodnik M. Zhu Y. Langhi L. G. P. Tchkonia T. Krüger P. Fielder E. et al (2019). Obesity-induced cellular senescence drives anxiety and impairs neurogenesis. Cell Metab.29 (5), 1233–1077.e8. 10.1016/j.cmet.2019.01.013

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 134

  Olivieri F. Albertini M. C. Orciani M. Ceka A. Cricca M. Procopio A. D. et al (2015). DNA damage response (DDR) and senescence: shuttled inflamma-miRNAs on the stage of inflamm-aging. Oncotarget6 (34), 35509–35521. 10.18632/oncotarget.5899

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 135

  Orjalo A. V. Bhaumik D. Gengler B. K. Scott G. K. Campisi J. (2009). Cell surface-bound IL-1alpha is an upstream regulator of the senescence-associated IL-6/IL-8 cytokine network. Proc. Natl. Acad. Sci.106 (40), 17031–17036. 10.1073/pnas.0905299106

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 136

  Ortiz-Montero P. Londoño-Vallejo A. Vernot J. P. (2017). Senescence-associated IL-6 and IL-8 cytokines induce a self- and cross-reinforced senescence/inflammatory milieu strengthening tumorigenic capabilities in the MCF-7 breast cancer cell line. Cell Commun. Signal15 (1), 17. 10.1186/s12964-017-0172-3

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 137

  Pacifico J. Geerlings M. A. J. Reijnierse E. M. Phassouliotis C. Lim W. K. Maier A. B. (2020). Prevalence of sarcopenia as a comorbid disease: a systematic review and meta-analysis. Exp. Gerontol.131, 110801. 10.1016/j.exger.2019.110801

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 138

  Park C. Cha H. J. Kim D. H. Kwon C. Y. Park S. H. Hong S. H. et al (2023). Fisetin protects C2C12 mouse myoblasts from oxidative stress-induced cytotoxicity through regulation of the Nrf2/HO-1 signaling. J. Microbiol. Biotechnol.33 (5), 591–599. 10.4014/jmb.2212.12042

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 139

  Passos J. F. Saretzki G. Ahmed S. Nelson G. Richter T. Peters H. et al (2007). “Mitochondrial dysfunction accounts for the stochastic heterogeneity in telomere-dependent senescence,”PLoS Biol. Editor De LangeT.5 (5) e110. 10.1371/journal.pbio.0050110

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 140

  Pawlikowski B. Vogler T. O. Gadek K. Olwin B. B. (2017). Regulation of skeletal muscle stem cells by fibroblast growth factors. Dev. Dyn.246 (5), 359–367. 10.1002/dvdy.24495

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 141

  Perez K. Ciotlos S. McGirr J. Limbad C. Doi R. Nederveen J. P. et al (2022). Single nuclei profiling identifies cell specific markers of skeletal muscle aging, frailty, and senescence. Aging14 (23), 9393–9422. 10.18632/aging.204435

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 142

  Pundlik S. S. Barik A. Venkateshvaran A. Sahoo S. S. Jaysingh M. A. Math R. G. et al (2024). “Senescent cells inhibit mouse myoblast differentiation via the SASP-Lipid 15d-PGJ2 mediated modification and control of HRas,”eLife. Editors NRS.HuangC. L. H.13RP95229. 10.7554/eLife.95229

  • CrossRef
  • Google Scholar

• 143

  Quijano C. Cao L. Fergusson M. M. Romero H. Liu J. Gutkind S. et al (2012). Oncogene-induced senescence results in marked metabolic and bioenergetic alterations. Cell Cycle11 (7), 1383–1392. 10.4161/cc.19800

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 144

  Reid M. B. Li Y. P. (2001). Tumor necrosis factor-α and muscle wasting: a cellular perspective. Respir. Res.2 (5), 269–272. 10.1186/rr67

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 145

  Rocheteau P. Gayraud-Morel B. Siegl-Cachedenier I. Blasco M. A. Tajbakhsh S. (2012). A subpopulation of adult skeletal muscle stem cells retains all template DNA strands after cell division. Cell148 (1–2), 112–125. 10.1016/j.cell.2011.11.049

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 146

  Rodier F. Coppé J. P. Patil C. K. Hoeijmakers W. A. M. Muñoz D. P. Raza S. R. et al (2009). Persistent DNA damage signalling triggers senescence-associated inflammatory cytokine secretion. Nat. Cell Biol.11 (8), 973–979. 10.1038/ncb1909

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 147

  Rudnicki M. A. Schnegelsberg P. N. J. Stead R. H. Braun T. Arnold H. H. Jaenisch R. (1993). MyoD or Myf-5 is required for the formation of skeletal muscle. Cell75 (7), 1351–1359. 10.1016/0092-8674(93)90621-v

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 148

  Sahu A. Clemens Z. J. Shinde S. N. Sivakumar S. Pius A. Bhatia A. et al (2021). Regulation of aged skeletal muscle regeneration by circulating extracellular vesicles. Nat. Aging1 (12), 1148–1161. 10.1038/s43587-021-00143-2

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 149

  Sapieha P. Mallette F. A. (2018). Cellular senescence in postmitotic cells: beyond growth arrest. Trends Cell Biol.28 (8), 595–607. 10.1016/j.tcb.2018.03.003

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 150

  Sasaki K. ichiro Fukumoto Y. (2022). Sarcopenia as a comorbidity of cardiovascular disease. J. Cardiol.79 (5), 596–604. 10.1016/j.jjcc.2021.10.013

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 151

  Saul D. Kosinsky R. L. Atkinson E. J. Doolittle M. L. Zhang X. LeBrasseur N. K. et al (2022). A new gene set identifies senescent cells and predicts senescence-associated pathways across tissues. Nat. Commun.13 (1), 4827. 10.1038/s41467-022-32552-1

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 152

  Schaap L. A. Pluijm S. M. F. Deeg D. J. H. Visser M. (2006). Inflammatory markers and loss of muscle mass (sarcopenia) and strength. Am. J. Med.119 (6), 526.e9–526.e5.26E17. 10.1016/j.amjmed.2005.10.049

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 153

  Severino V. Alessio N. Farina A. Sandomenico A. Cipollaro M. Peluso G. et al (2013). Insulin-like growth factor binding proteins 4 and 7 released by senescent cells promote premature senescence in mesenchymal stem cells. Cell Death Dis.4 (11), e911. 10.1038/cddis.2013.445

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 154

  Shimi T. Butin-Israeli V. Adam S. A. Hamanaka R. B. Goldman A. E. Lucas C. A. et al (2011). The role of nuclear lamin B1 in cell proliferation and senescence. Genes Dev.25 (24), 2579–2593. 10.1101/gad.179515.111

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 155

  Sidler C. Kovalchuk O. Kovalchuk I. (2017). Epigenetic regulation of cellular senescence and aging. Front. Genet.26 (8(SEP). 10.3389/fgene.2017.00138

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 156

  Sinha M. Jang Y. C. Oh J. Khong D. Wu E. Y. Manohar R. et al (2014). Restoring systemic GDF11 levels reverses age-related dysfunction in mouse skeletal muscle. Science344 (6184), 649–652. 10.1126/science.1251152

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 157

  Solovyeva E. M. Ibebunjo C. Utzinger S. Eash J. K. Dunbar A. Naumann U. et al (2021). New insights into molecular changes in skeletal muscle aging and disease: differential alternative splicing and senescence. Mech. Ageing Dev.197, 111510. 10.1016/j.mad.2021.111510

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 158

  Soriano‐Arroquia A. Gostage J. Xia Q. Bardell D. McCormick R. McCloskey E. et al (2021). miR‐24 and its target gene Prdx6 regulate viability and senescence of myogenic progenitors during aging. Aging Cell24 (July), e13475–16. 10.1111/acel.13475

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 159

  Sosa P. Alcalde-Estevez E. Plaza P. Troyano N. Alonso C. Martínez-Arias L. et al (2018). Hyperphosphatemia promotes senescence of myoblasts by impairing autophagy through ilk overexpression, A possible mechanism involved in sarcopenia. Aging Dis.9 (5), 769–784. 10.14336/AD.2017.1214

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 160

  Sousa-Victor P. Muñoz-Cánoves P. (2016). Regenerative decline of stem cells in sarcopenia. Mol. Asp. Med.50, 109–117. 10.1016/j.mam.2016.02.002

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 161

  Sousa-Victor P. Gutarra S. García-Prat L. Rodriguez-Ubreva J. Ortet L. Ruiz-Bonilla V. et al (2014). Geriatric muscle stem cells switch reversible quiescence into senescence. Nature506 (7488), 316–321. 10.1038/nature13013

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 162

  Sousa-Victor P. García-Prat L. Muñoz-Cánoves P. (2021). Control of satellite cell function in muscle regeneration and its disruption in ageing. Nat. Rev. Mol. Cell Biol.0123456789. 10.1038/s41580-021-00421-2

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 163

  Steele A. P. Syroid A. L. Mombo C. Raveetharan S. Rebalka I. A. Hawke T. J. (2024). Isolation of a persistently quiescent muscle satellite cell population. Am. J. Physiol. Cell Physiol.327 (2), C415–C422. 10.1152/ajpcell.00231.2024

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 164

  Sturmlechner I. Sine C. C. Jeganathan K. B. Zhang C. Fierro Velasco R. O. Baker D. J. et al (2022). Senescent cells limit p53 activity via multiple mechanisms to remain viable. Nat. Commun.13 (1), 3722. 10.1038/s41467-022-31239-x

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 165

  Sugihara H. Teramoto N. Yamanouchi K. Matsuwaki T. Nishihara M. (2018). Oxidative stress-mediated senescence in mesenchymal progenitor cells causes the loss of their fibro/adipogenic potential and abrogates myoblast fusion. Aging10 (4), 747–763. 10.18632/aging.101425

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 166

  Takebayashi S. ichiro Tanaka H. Hino S. Nakatsu Y. Igata T. Sakamoto A. et al (2015). Retinoblastoma protein promotes oxidative phosphorylation through upregulation of glycolytic genes in oncogene-induced senescent cells. Aging Cell14 (4), 689–697. 10.1111/acel.12351

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 167

  Tai H. Wang Z. Gong H. Han X. Zhou J. Wang X. et al (2017). Autophagy impairment with lysosomal and mitochondrial dysfunction is an important characteristic of oxidative stress-induced senescence. Autophagy13 (1), 99–113. 10.1080/15548627.2016.1247143

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 168

  Takasugi M. (2018). Emerging roles of extracellular vesicles in cellular senescence and aging. Aging Cell17 (2), e12734–e12738. 10.1111/acel.12734

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 169

  Takasugi M. Okada R. Takahashi A. Virya Chen D. Watanabe S. Hara E. (2017). Small extracellular vesicles secreted from senescent cells promote cancer cell proliferation through EphA2. Nat. Commun.8 (1), 15729. 10.1038/ncomms15728

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 170

  Tanaka Y. Takahashi A. (2021). Senescence-associated extracellular vesicle release plays a role in senescence-associated secretory phenotype (SASP) in age-associated diseases. J. Biochem. (Tokyo)169 (2), 147–153. 10.1093/jb/mvaa109

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 171

  Terlecki-Zaniewicz L. Lämmermann I. Latreille J. Bobbili M. R. Pils V. Schosserer M. et al (2018). Small extracellular vesicles and their miRNA cargo are anti-apoptotic members of the senescence-associated secretory phenotype. Aging10 (5), 1103–1132. 10.18632/aging.101452

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 172

  Valadi H. Ekström K. Bossios A. Sjöstrand M. Lee J. J. Lötvall J. O. (2007). Exosome-mediated transfer of mRNAs and microRNAs is a novel mechanism of genetic exchange between cells. Nat. Cell Biol.9 (6), 654–659. 10.1038/ncb1596

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 173

  van Deursen J. M. (2014). The role of senescent cells in ageing. Nature509 (7501), 439–446. 10.1038/nature13193

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 174

  Verdijk L. B. Koopman R. Schaart G. Meijer K. Savelberg HHCM van Loon L. J. C. (2007). Satellite cell content is specifically reduced in type II skeletal muscle fibers in the elderly. Am. J. Physiol. Endocrinol. Metab.292 (1), E151–E157. 10.1152/ajpendo.00278.2006

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 175

  Verdijk L. B. Snijders T. Drost M. Delhaas T. Kadi F. Van Loon L. J. C. (2014). Satellite cells in human skeletal muscle; from birth to old age. Age36 (2), 545–547. 10.1007/s11357-013-9583-2

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 176

  Visser M. Pahor M. Taaffe D. R. Goodpaster B. H. Simonsick E. M. Newman A. B. et al (2002). Relationship of Interleukin-6 and tumor necrosis Factor-α with muscle mass and muscle strength in elderly men and women: the health ABC study. J. Gerontol. Ser. A57 (5), M326–M332. 10.1093/gerona/57.5.m326

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 177

  von Zglinicki T. Wan T. Miwa S. (2021). Senescence in post-mitotic cells: a driver of aging?Antioxid. Redox Signal34 (4), 308–323. 10.1089/ars.2020.8048

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 178

  Wada M. R. Inagawa-Ogashiwa M. Shimizu S. Yasumoto S. Hashimoto N. (2002). Generation of different fates from multipotent muscle stem cells. Dev. Camb Engl.129 (12), 2987–2995. 10.1242/dev.129.12.2987

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 179

  Wang E. (1995). Senescent human fibroblasts resist programmed cell death, and failure to suppress bcl2 is involved. Cancer Res.55 (11), 2284–2292.

  • Pubmed Abstract
  • Google Scholar

• 180

  Wang C. Jurk D. Maddick M. Nelson G. Martin-Ruiz C. Von Zglinicki T. (2009). DNA damage response and cellular senescence in tissues of aging mice. Aging Cell8 (3), 311–323. 10.1111/j.1474-9726.2009.00481.x

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 181

  Wang B. Han J. Elisseeff J. H. Demaria M. (2024). The senescence-associated secretory phenotype and its physiological and pathological implications. Nat. Rev. Mol. Cell Biol.25 (12), 958–978. 10.1038/s41580-024-00727-x

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 182

  Warnier M. Flaman J. M. Chouabe C. Wiel C. Gras B. Griveau A. et al (2018). The SCN9A channel and plasma membrane depolarization promote cellular senescence through Rb pathway. Aging Cell17 (3), e12736. 10.1111/acel.12736

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 183

  Wen X. Klionsky D. J. (2016). Autophagy is a key factor in maintaining the regenerative capacity of muscle stem cells by promoting quiescence and preventing senescence. Autophagy12 (4), 617–618. 10.1080/15548627.2016.1158373

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 184

  White J. P. Billin A. N. Campbell M. E. Russell A. J. Huffman K. M. Kraus W. E. (2018). The AMPK/p27Kip1 axis regulates autophagy/apoptosis decisions in aged skeletal muscle stem cells. Stem Cell Rep.11 (2), 425–439. 10.1016/j.stemcr.2018.06.014

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 185

  Wiley C. D. Campisi J. (2021). The metabolic roots of senescence: mechanisms and opportunities for intervention. Nat. Metab.3 (10), 1290–1301. 10.1038/s42255-021-00483-8

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 186

  Wiley C. D. Velarde M. C. Lecot P. Liu S. Sarnoski E. A. Freund A. et al (2016). Mitochondrial dysfunction induces senescence with a distinct secretory phenotype. Cell Metab.23 (2), 303–314. 10.1016/j.cmet.2015.11.011

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 187

  Wiley C. D. Flynn J. M. Morrissey C. Lebofsky R. Shuga J. Dong X. et al (2017). Analysis of individual cells identifies cell-to-cell variability following induction of cellular senescence. Aging Cell16 (5), 1043–1050. 10.1111/acel.12632

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 188

  Wiley C. D. Brumwell A. N. Davis S. S. Jackson J. R. Valdovinos A. Calhoun C. et al (2019). Secretion of leukotrienes by senescent lung fibroblasts promotes pulmonary fibrosis. JCI Insight4 (24), e130056. 10.1172/jci.insight.130056

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 189

  Wiley C. D. Sharma R. Davis S. S. Lopez-Dominguez J. A. Mitchell K. P. Wiley S. et al (2021). Oxylipin biosynthesis reinforces cellular senescence and allows detection of senolysis. Cell Metab.33 (6), 1124–1136.e5. 10.1016/j.cmet.2021.03.008

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 190

  Xu M. Pirtskhalava T. Farr J. N. Weigand B. M. Palmer A. K. Weivoda M. M. et al (2018). Senolytics improve physical function and increase lifespan in old age. Nat. Med.24 (8), 1246–1256. 10.1038/s41591-018-0092-9

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 191

  Yamamoto M. Legendre N. P. Biswas A. A. Lawton A. Yamamoto S. Tajbakhsh S. et al (2018). Loss of MyoD and Myf5 in skeletal muscle stem cells results in altered myogenic programming and failed regeneration. Stem Cell Rep.10 (3), 956–969. 10.1016/j.stemcr.2018.01.027

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 192

  Yim W. W. Y. Mizushima N. (2020). Lysosome biology in autophagy. Cell Discov.6 (1), 6–12. 10.1038/s41421-020-0141-7

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 193

  Yousefzadeh M. J. Zhu Y. McGowan S. J. Angelini L. Fuhrmann-Stroissnigg H. Xu M. et al (2018). Fisetin is a senotherapeutic that extends health and lifespan. eBioMedicine36, 18–28. 10.1016/j.ebiom.2018.09.015

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 194

  Zhang X. Habiballa L. Aversa Z. Ng Y. E. Sakamoto A. E. Englund D. A. et al (2022a). Characterization of cellular senescence in aging skeletal muscle. Nat. Aging2 (7), 601–615. 10.1038/s43587-022-00250-8

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 195

  Zhang Y. Ye Y. Tang X. Wang H. Tanaka T. Tian R. et al (2022b). CCL17 acts as a novel therapeutic target in pathological cardiac hypertrophy and heart failure. J. Exp. Med.219 (8), e20200418. 10.1084/jem.20200418

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 196

  Zhang Y. Tang X. Wang Z. Wang L. Chen Z. Qian J. Y. et al (2023). The chemokine CCL17 is a novel therapeutic target for cardiovascular aging. Signal Transduct. Target Ther.8 (1), 157. 10.1038/s41392-023-01363-1

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 197

  Zhou J. Chen H. Wang Q. Chen S. Wang R. Wang Z. et al (2022). Sirt1 overexpression improves senescence-associated pulmonary fibrosis induced by vitamin D deficiency through downregulating IL-11 transcription. Aging Cell21 (8), e13680. 10.1111/acel.13680

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 198

  Zhu Y. Tchkonia T. Pirtskhalava T. Gower A. C. Ding H. Giorgadze N. et al (2015). The achilles’ heel of senescent cells: from transcriptome to senolytic drugs. Aging Cell14 (4), 644–658. 10.1111/acel.12344

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 199

  Zhu Y. Tchkonia T. Fuhrmann‐Stroissnigg H. Dai H. M. Ling Y. Y. Stout M. B. et al (2016). Identification of a novel senolytic agent, navitoclax, targeting the Bcl‐2 family of anti‐apoptotic factors. Aging Cell15 (3), 428–435. 10.1111/acel.12445

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 200

  Zhu Y. Doornebal E. J. Pirtskhalava T. Giorgadze N. Wentworth M. Fuhrmann-Stroissnigg H. et al (2017). New agents that target senescent cells: the flavone, fisetin, and the BCL-XL inhibitors, A1331852 and A1155463. Aging.9 (3), 955–963. 10.18632/aging.101202

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 201

  Zhu P. Zhang C. Gao Y. Wu F. Zhou Y. Wu W. S. (2019). The transcription factor slug represses p16Ink4a and regulates murine muscle stem cell aging. Nat. Commun.10 (1), 2568. 10.1038/s41467-019-10479-4

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 202

  Zhu G. Z. Zhao K. Li H. Z. Wu D. Z. Chen Y. B. Han D. et al (2024). Melatonin ameliorates age-related sarcopenia by inhibiting fibrogenic conversion of satellite cell. Mol. Med.30 (1), 238–15. 10.1186/s10020-024-00998-2

  • Pubmed Abstract
  • CrossRef
  • Google Scholar