p16 in Different Tissues and Organs: Comparison
View Latest Version
Please note this is a comparison between Version 2 by Amina Yu and Version 1 by Kay-Dietrich Wagner.

P16 is a tumor suppressor gene, which has been termed with several names such as the multiple tumor suppressor-1 (MTS-1), the inhibitor of cyclin-dependent kinase 4a (INK4A), or the cyclin-dependent kinase inhibitor 2a (CDKN2A). The human p16 gene is located on the short arm of chromosome (9p21.3). The p16 transcript is composed of three exons which encode 156 amino acids. The use of an alternative reading frame generates the human p14Arf protein (p19Arf in mice). In several selected tissues and organs, including skin, bones, lungs, brain, heart, kidney, and liver, weit is intended to address the well-known function of p16 in senescence and aging, and discuss several functions of p16, which might be more related to its classical role as a cell cycle regulator.

  • aging
  • cancer
  • development
  • p16

21. The P16 Gene

The CDKN2A gene belongs to the INK4 genes family. CDKN2A encodes for p16Ink4A and p14ARF (p19Arf in mice), while CDKN2B encodes for p15Ink4B, CDKN2C for p18Ink4D, and CDKN2D for p19Ink4D. They share biological properties in cell cycle regulation and tumor suppression [56,57][1][2]. The p16INK4A structure consists of five exons E1β, E1α, E2, E2γ, and E3. Alternative splicing generates four different transcript variants including p16 (E1α, E2, and E3), p19Arf (E1β, E2, and E3), (the murine orthologue of the human p14ARF), in addition to p16γ and p12. Thus, the difference between p16 and p19ARF transcript variants lies within the alternative splicing of E1α versus E1β [58,59][3][4] (Figure 1).
Life 12 01332 g001 550
Figure 1. The structure of the INK4A locus gives rise to several transcripts through alternative splicing. P16INK4A and p19ARF are two transcripts of 3 exons which differ only in the first exon that is E1α for p16 and E1β for p19ARF.

2. In the Skin

The skin is the largest tissue in the human body. It serves as a physical barrier to both biological and nonbiological threats. Being exposed to the outside environment places the skin in direct contact with environmental hazards, making it extremely vulnerable. The skin is made up of two layers: the outer epidermis, which is divided into four sublayers with keratinocytes predominating in the spinous, granular, and cornfield sublayers, and pigment-producing melanocytes that confer photoprotection in the basal sublayer. The underlying dermis contains connective tissue with fibroblasts, collagen, and elastin as well as sebaceous and sweat glands and is connected to the epidermis by the dermal epidermal joint (DEJ) [98]. Skin aging is caused by both intrinsic (genetic, time, etc.) and extrinsic (pollution, UV exposure, sunlight, etc.) factors, and it has both biological and functional implications.

2. In the Skin

The skin is the largest tissue in the human body. It serves as a physical barrier to both biological and nonbiological threats. Being exposed to the outside environment places the skin in direct contact with environmental hazards, making it extremely vulnerable. The skin is made up of two layers: the outer epidermis, which is divided into four sublayers with keratinocytes predominating in the spinous, granular, and cornfield sublayers, and pigment-producing melanocytes that confer photoprotection in the basal sublayer. The underlying dermis contains connective tissue with fibroblasts, collagen, and elastin as well as sebaceous and sweat glands and is connected to the epidermis by the dermal epidermal joint (DEJ) [5]. Skin aging is caused by both intrinsic (genetic, time, etc.) and extrinsic (pollution, UV exposure, sunlight, etc.) factors, and it has both biological and functional implications. Aged skin has thinner epidermis, dermis, and DEJ than younger skin, which is due to keratinocytes’ decreased proliferation and renewal ability [6][7][8][9].

Aged skin has thinner epidermis, dermis, and DEJ than younger skin, which is due to keratinocytes’ decreased proliferation and renewal ability [25,99,100,101].
As ma major biomarkers of senescence, both the SA-β-gal and p16 determination has shown elevated expression upon in vitro exposure of fibroblasts and keratinocytes to UV light [102,103,104][10][11][12]. Furthermore, telomere shortening, DNA damage, and UV exposure increased the activity of the p16/pRB and P19ARF/p53/P21 cascades, resulting in an accumulation of senescent cells and skin stem cell dysfunction and loss of regeneration capacity [101][9]. An in vivo study, on the other hand, claimed that UV light exposure has accelerated cellular senescence by increasing p21 expression [104][12].
In contrast to the previous results, the presence of p16 has been shown to play an important role in several biological processes that are beneficial to the skin. Starting with its tumor suppression function, p16 inactivation due to mutation or promoter methylation has been linked to a variety of cancers, including familial and sporadic melanoma [105,106,107,108][13][14][15][16]. These studies identified 55 out of 60 melanoma cell lines that were dependent on complete or partial p16 aberration, implicating this pathway in the development of melanomas. Furthermore, the level of p16 expression could be used as a melanoma predictive and prognostic biomarker. In other words, lower p16 levels were associated with higher Ki67 expression as a proliferation marker, and metastatic melanoma lesions were associated with even lower p16 levels and predicted poor patient survival [109][17]. Benign nevi had higher p16 levels than nonmetastatic melanoma, which had even higher p16 levels than metastatic melanoma [110][18]. Furthermore, in primary mouse fibroblasts (PMFs), human melanocytes, and a human melanoma cell line (A375), the loss of p16 correlated with increased mitochondrial mass, attenuated respiration, and altered morphology associated with augmented superoxide production and higher cellular motility. Forced p16 expression restored mitochondrial homeostasis, dynamics, and motility in a CDK4/pRB independent pathway [111][19]. Surprisingly, oxidative stress-induced p16 has attenuated ROS production in skin in vivo and in vitro. In addition, elevated intracellular ROS and DNA damage were obtained in p16-deficient cells. This was restored in skin fibroblasts transduced with p16 using lentivirus [72][20]. These findings suggest a pRB-independent tumor suppression function of p16. As another mechanism, p16 has been found to transactivate the promoter of the tumor suppressor miRNAs, miRNA-141 and miRNA-146b-5p, in melanocyte through physical interaction with the transcription factor Sp1 and CDK4, via the p16 fourth ankyrin repeat. Mutation in this ankyrin repeat attenuated Sp1 binding and miRNA-141 and miRNA-146b-5p transactivation without affecting the expression level of Sp1 [112][21]. In addition, this p16–Sp1–CDK4 interaction and consequent miRNA-141 and miRNA-146b-5p transactivation has also been implicated in cellular response to UV-radiation-induced damage and apoptosis.
P16 has been shown to be an important factor in wound healing. Endothelial cells and fibroblasts were identified as p16-positive cells at the site of injury in the p16-3MR mouse model a few days after injury. These transiently appearing senescent cells aimed to accelerate wound closure by inducing myofibroblast differentiation via platelet-derived growth factor AA secretion as part of the SASP [43][22]. Elimination of these cells delayed the wound healing process. The matricellular protein CCN1 has been identified as a key player in the induction of fibroblast senescence at the wound healing margins. By inducing DNA damage and p53 activity, CCN1 induces oxidative stress and provokes p16 upregulation, which leads to fibroblast senescence and antifibrotic gene activation [113][23]. Furthermore, coexpression and activation of the laminin 5/p16 response has been identified in migrating keratinocytes. The laminin 5/p16 response caused hypermotility and growth arrest in keratinocytes, leading to wound re-epithelialization [44][24]. This pathway has also been identified in critical stage neoplastic progression as a tumor suppressing pathway. This might suggest a protective effect of the induced p16 upregulation upon the exposure of skin to UV radiation [114][25].
Moreover, p16-orchestrated expression is required for stem cell self-renewal and differentiation. More precisely, p16 repression by epigenetic regulators is indispensable for stem cells proliferation. On the contrary, its promoter epigenetic regulation and orchestrated expression level have been found crucial for keratinocyte differentiation beside many other differentiation genes [115,116,117,118,119][26][27][28][29][30]. However, p16 seems not causal for terminal differentiation as it is expressed during early embryonic development [120][31], but still the balance between growth and differentiation requires a balanced expression of p16 and other cell cycle regulators [116,117,118,119][27][28][29][30]. For instance, Id-1, Id-2, and Id-3 are repressors of p16 and are upregulated in dividing keratinocytes, whereas they become downregulated in differentiated cells [121][32]. Activators of p16 transcription promoted keratinocyte differentiation via acting on epidermal differentiation complex genes [46][33]. Therefore, unravelling the precise mechanism underlying p16 regulation of expression might provide a targeted approach which confers maintenance of epidermis regenerative capacity and avoids premature skin aging or cancer development (Figure 32).
Life 12 01332 g003 550
Figure 32. Schematic illustration that summarizes the major functions or implications of p16 in homeostasis, pathophysiology, and cancer of different organs.

3. In the Bones

Two major types of cells are involved in maintaining skeletal homeostasis: osteoblasts, which are derived from osteoprogenitor cells and are in charge of bone growth, mineralization, and remodeling, and osteoclasts, which are descended from myeloid lineages and mediate bone resorption and breakdown [122][34]. Osteocytes are the most prevalent long-lived cell type in bone matrix and are in charge of maintenance of bone mass [123][35]. Skeletal aging is characterized by bone mass loss and is a significant risk factor for osteoporosis because it results from an increase in osteoclasts and a decrease in osteoblasts count [124,125,126,127][36][37][38][39]. Cellular senescence has been linked to bone aging and the development of aging-related osteo-pathologies [128][40]. More precisely, senescent osteocytes have been detected in aging bones with increased expression of p16.
In contrast to osteocytes, senescent osteoblasts are characterized by increased expression of p21 only [123,126,129,130,131][35][38][41][42][43]. Moreover, the selective elimination of p16-expressing cells using INK-ATTACK transgene resulted in increased bone mass in 20 months old mice [132][44]. Furthermore, using the p16-3MR transgene, which is based on the elimination of P16-expressing cells upon treatment with ganciclovir (GCV), has effectively abrogated age-related increases in osteoclastogenesis of the myeloid lineage but had no effect on bone formation. This might indicate that p16, rather than direct targeting of senescent osteocytes, contributes to osteoclastogenic potential without major impact on age-related bone loss [133][45].
However, other implications of p16 have been demonstrated in bone. P16 degradation by the ubiquitinated regulator UBE2S is an important step in the progression of prostate cancer bone metastasis [134][46]. Furthermore, patients with p16-positive oropharyngeal squamous cell carcinoma had a higher incidence of bone metastasis than p16-negative patients [135][47]. Lower expression of p16 in osteosarcoma patients was correlated with reduced response to primary chemotherapy [136][48], which, therefore, shows the importance of p16 as a prognostic and predictive biomarker and therapeutic target for cancer and metastasis.
Aside from p16 in cancer, although only p21-positive cells were able to prevent radiation-induced osteoporosis [86][49], p16 deletion inhibited oxidative stress, osteocyte senescence, and osteoclastic bone resorption, which led to osteogenesis and osteoblastic bone formation, indicating a promising mechanism to prevent estrogen deficiency-induced osteoporosis [137][50]. Furthermore, p16 deletion promoted migration, proliferation, and differentiation of bone marrow mesenchymal stem cells (BM-MSCs) and chondrocytes. It also stimulated osteoblastogenesis and vascularization, which improved bone fracture healing. Consequently, p16 modification might offer a novel strategy for treating fractured bones in elderly patients [138][51] (Figure 32).

4. In the Lungs

Cellular senescence and aging have both been linked to increased lung damage and functional impairment [139][52]. Growing evidence suggested aging as another determinant of the chronic obstructive pulmonary disease (COPD) and showed higher prevalence of the disease in elderly [140,141,142][53][54][55]. Similarly, even though there are no certain causes of idiopathic pulmonary fibrosis (IPF), aging associated with cellular senescence and p16 overexpression has emerged as a main risk factor [143,144][56][57].
Cigarette smoking (CS) is a major risk factor attributed to COPD [145][58]. CS can alter cellular proliferation and induce apoptosis, reactive oxygen species production, and promote oxidative stress, cause DNA damage, and trigger cellular senescence [146,147][59][60]. Furthermore, mice exposed to chronic cigarette smoking at both young and old ages showed increased activation of the senescence marker beta-galactosidase as well as upregulation of p16 compared to their respective air-exposed controls. Older air-exposed mice had higher levels of beta-galactosidase and p16 than younger mice. Therefore, CS-induced senescence and natural-aging-associated senescence are both affected by the p16 pathway [148][61]. This was confirmed in human COPD patients who had higher p16 expression compared to normal smokers and nonsmokers [149][62]. Furthermore, after CS exposure, wild type mice had more senescent alveolar type II (AECII) epithelial cells than p16 knockout mice, which had normal pulmonary function. Moreover, p16 deletion has rescued the adverse effects induced by CS in the lungs via the insulin growth factor1 (IGF1)/Akt1 signaling pathway [149][62].
However, p16 expression is a differentiation key between cervical squamous cell carcinoma (SCC) with pulmonary metastasis and pulmonary SCC. Immunohistochemistry of both cervical SCC without and with pulmonary metastasis has shown an intense staining of p16 in almost all cases studied. On the contrary, cases with pulmonary SCC demonstrated p16 expression in 7 out of 33 cases, 3 of which showed weak p16 staining. This implies the usefulness of p16 as a distinguishing marker between cervical SCC with lung metastasis and pulmonary SCC [150][63]. Furthermore, the fact that aberrant p16 methylation occurs at early stages of lung cancer renders p16 an early diagnostic biomarker for monitoring and prevention [151][64]. Moreover, p16 low expression and gene mutation were associated with early and late stage nonsmall cells lung carcinoma (NSCLC), respectively [152,153][65][66]. As a result, it has been identified as a predictable prognostic factor in NSCLC, particularly at the early stage.
On the other hand, p16 expression is not only linked with disease progression but also with lung protection. P16 loss was linked with poor survival after lung injury. In addition, p16 expression was found to be crucial for protection of lung epithelium against oncogenic stress and lung injury [154][67]. Moreover, injured p16-positive mesenchymal cells enhanced epithelial progenitor proliferation, whereas deletion of p16 attenuated normal epithelial repair in the lungs [155][68]. Furthermore, prevalent usefulness was demonstrated for p16 as a target for COPD therapy. Higher p16 expression was found in human COPD lungs compared to normal patients, and when CS induced impaired pulmonary function and augmented emphysema in WT mice, p16 knockout mice exhibited normal pulmonary function with reduced emphysema and increased alveolar progenitor proliferation [149][62] (Figure 32).

5. In the Brain

Aging-induced p16 overexpression and cellular senescence have been linked to decreased subventricular zone progenitor proliferation and neurogenesis of the olfactory bulb and to diminished multipotent progenitor cell frequency and self-renewal potency [156][69]. Moreover, chronic accumulation of senescent cells and the resulting inflammation in the brain has been linked to the development of Alzheimer’s disease (AD) and other neurodegenerative diseases [157,158][70][71]. In two out of five AD models, Dorigatti et al. [159][72] found evidence of cellular senescence marked by a significant increase in p16, p21, and p53 expression, as well as increased SASPs expression and beta-galactosidase activity [159][72]. Another study found that tau-containing neurofibrillary tangles (NFTs), a hallmark of Alzheimer’s disease, are age-dependent and strongly associated with senescence induction and upregulation of p16 and p21 [160,161][73][74]. Nonetheless, astrocytes play an important role in neuronal homeostasis and functions, and, as we age, they undergo senescence in response to multiple stresses, resulting in impaired brain function [162,163,164,165][75][76][77][78].
As previously discussed for other tumors, unsurprisingly, p16 homozygous deletion was found in both primary glioblastoma and their derived xenografts [167][79]. In addition, p16-cdk4/cyclin D1-pRb pathway inactivation was found in the majority of glioblastomas [168][80]. P16 loss was linked to significantly poor outcome in all glioma patients, which indicates a predictive prognostic usefulness of p16 in brain tumors [169][81]. On the contrary, p16 null glioma cells demonstrated higher chemosensitivity to paclitaxel and topotecan compared to exogenous wild type p16 overexpression [170][82].
P16 overexpression has been shown to exert a protective function of neurons against CDK overexpression-induced apoptosis [171][83]. Moreover, increased expression of p16 and p21, induced by stress conditions, has protected female but not male astrocytes from transformation [172][84]. In another promising strategy, the selective elimination of p16-positive senescent astrocytes diminished cognitive impairment induced by whole brain irradiation [173][85]. Lastly, dihydromyricetin (DMY), through the downregulation of p16, p21, and p53, was able to inhibit oxidative stress and neuroinflammation and to attenuate brain aging and improve cognitive function in mice [174][86] (Figure 32).

6. In the Heart

Remarkable p16 expression and cellular senescence were found in cardiac chronological aging and heart failure [175,176][87][88]. For example, elevated p16 expression and beta-galactosidase activity were found in cardiomyocytes gathered from Langendorff heart perfusion with aging [91][89]. In addition to that, cardiac progenitor cells isolated from elderly (> 70 years old) people expressed high levels of p16 and SASPs, alongside shortened telomeres and increased SA-β-gal [92][90]. Furthermore, remarkable telomere shortening and senescent-associated increased p16 expression were found in cardiomyocytes isolated from old rats compared to younger ones [177][91]. Older patients with heart failure had higher p16 expression, which was associated with senescence and cell death, as well as shorter telomere length, when compared to healthy elderly people. This suggests that p16-induced senescence, telomere attrition, and cell death are features of heart failure in aging [176][88]. Furthermore, vascular smooth muscle cell (VSMC) senescence in atherosclerotic plaques was marked by increased p16, p21, and p53 expression in addition to increased beta-galactosidase activity [178][92].
The recovery of cardiac function and cardiac remodeling have been correlated with cardiac stem cell (CSCs) regeneration and differentiation ability [179,180][93][94]. Cellular senescence has an impact on CSCs and cardiac function, which might provide a concept of therapies by targeting senescent cells for cardiac functional improvement and extended lifespan in elderly people [179][93]. With aging, a significant portion of human CSCs become senescent with elevated expression of p16, SA-β-gal, and SASPs, which contribute to CSC senescence and impaired cardiac regeneration. However, INK-ATTAC or senolytic elimination of senescent CSCs reactivated resident CSCs and increased cardiomyocyte proliferation [179][93] reflecting the importance of p16-positive senescent CSCs as therapeutic approach for cardiac functional improvement. P16-positive cells that accumulate during adulthood have a negative impact on lifespan and promote age-dependent changes in the heart. The removal of p16-positive cells delayed age-related heart deterioration. Thus, the therapeutic removal of these cells may be an appealing approach to extend healthy lifespan [8][95].
On the contrary to the previous studies, the existence of p16 high cells detected in p16-CreERT2-tdTomato mouse model, was found indispensable for health span, and their elimination has induced cardiac fibrosis [83][96]. Furthermore, p16 overexpression has been detected in the infarction zone after myocardial infarction. The increased expression of p16 was associated with protected cardiac function and plays an important role for cardiac remodeling after myocardial infarction [181][97] (Figure 32).

7. In the Kidney

Several studies have linked p16 induction and subsequent cellular senescence to renal aging, diseases, and allograft rejection [182,183,184][98][99][100]. Age-dependent p16 upregulation in cortical tubular and interstitial cells was observed in humans. In addition, p16 and p27 expression were higher in the glomeruli, tubules, and interstitial cells of rejected grafts compared to normal kidneys [183][99]. Whether this reflects senescence as the underlying mechanism for chronic allograft rejection as suggested or might correspond to reduced proliferation and repair or to an increased immune reaction remains to be determined. In line with this, in human kidney specimens ranging from 8 weeks to 88 years of age, p16 induction was negatively correlated with the proliferation marker Ki-67 [185][101], which is in agreement with the role of p16 as a cell cycle inhibitor. Levels of p16 in glomerular and interstitial cells were significantly higher in kidneys with glomerular disease than in normal aged kidneys and kidneys with tubular interstitial nephritis. P16 expression was higher in kidneys with proteinuria, with fibrosis, or interstitial inflammation [186][102]. Whether this increased P16 expression is cause or consequence of glomerular disease remains an open question. Similarly, increased p16 expression was observed in kidneys of hypertensive animals and patients and kidneys with type 2 diabetic nephropathy [187,188][103][104]. Blood pressure lowering reduced p16 expression [187][103], which argues against a close relation between P16 and irreversible senescence in this model. Increased p16 expression has been reported in acute kidney injury (AKI) and in acute tubular necrosis (ATN) [189][105]. P16 deletion ameliorated ATN and improved kidney function in animal models [189][105]. Similarly, p16 deletion in Bmi-1-deficient mice rescued kidney aging features including function and structure, ameliorated tubulointerstitial fibrosis, and inhibited epithelial mesenchymal transition of renal interstitial fibroblasts [190][106] (Figure 32).

8. In the Liver

Although the majority of liver functions appear to be preserved with age, evidence of aging and cellular senescence associated with liver functional decline, reduced regenerative capacity, and diseases are well-documented [191,192,193][107][108][109]. P16 expression was higher in elderly hepatectomy patients compared to younger ones, and the increased p16 expression was associated with decreased liver regeneration [194][110]. This is in agreement with the attenuated proliferative response of hepatocytes in old rat liver compared to young animals [195][111]. P16 upregulation was observed in liver tissue and liver sinusoidal endothelial cells (LSEC) in an aged rat model compared to young animals [196][112]. The p16 CreERT2 tdTomato mouse model also demonstrated that p16 high cells were detectable in the liver, and that they were enriched with aging. The majority of the P16-positive liver cells found were vascular endothelial, and their removal caused steatohepatitis and perivascular tissue fibrosis [83,197][96][113]. This is compatible with higher p16 expression level of liver endothelial cells compared to nonendothelial cells demonstrated in our recent study [120][31].
With respect to liver metabolism, the extra copy of p16 carried by the “Super-INK4A/ARF” mouse model prevented the development of glucose intolerance with aging. Instead, increased activation of insulin receptors and high insulin sensitivity were obtained. This reveals a protective role of INK4A/ARF locus against age-induced insulin resistance [198][114], whereas increased insulin secretion, attenuated insulin sensitivity, and reduced hepatic insulin clearance were observed upon loss of function mutation of the Cdkn2a gene [199][115]. On the contrary, p16 deficiency improved fasting-activated glucose production in the liver, via the activation of PKA-CREB-PGC1α [200][116]. Altogether, these studies show the importance of p16 in glucose homeostasis. However, p16 has not been only implicated in glucose but also in fat metabolism. P16 has been found to regulate fasting-induced fatty acid oxidation and lipid droplet accumulation in the liver in vivo and in vitro. In addition, p16 deficiency was correlated with increased expression of fatty acids catabolism genes in primary hepatocytes [201][117]. Furthermore, p16-positive senescent cell accumulation has been correlated with hepatic fat deposition and steatosis. Elimination of these cells in the INK-ATTAC mouse model or senolytics treatment (dasatinib plus quercetin) attenuated liver fibrosis [88][118]. However, the feedback loop between lipid accumulation and increased p16 expression remains intriguing. Senescence in hepatocytes triggered fat accumulation [88][118], while high fat diet provoked significantly elevated p16 expression [202][119].
Nonetheless, several studies have also described p16 functions in liver cancers. P16 hypermethylation and consequent p16 inactivation has a pivotal role in the development of hepatocellular carcinoma and liver cirrhosis [205][120]. Wong et al. reported aberrantly methylated p16 in the plasma of liver cancer patients, suggesting the usefulness of these circulating liver-cancer-methylated DNA for the monitoring of tumors [206][121]. Therefore, all this information combined suggests that p16 regulation and meticulously unravelling the molecular mechanisms regulating p16 expression in liver physiology and liver pathologies require further elucidation and could unveil novel therapeutic strategies for maintaining normal liver function and extending lifespan (Figure 32).

References

  1. Serrano, M. The tumor suppressor protein p16INK4a. Exp. Cell Res. 1997, 237, 7–13.
  2. Komata, T.; Kanzawa, T.; Takeuchi, H.; Germano, I.M.; Schreiber, M.; Kondo, Y.; Kondo, S. Antitumour effect of cyclin-dependent kinase inhibitors (p16(INK4A), p18(INK4C), p19(INK4D), p21(WAF1/CIP1) and p27(KIP1)) on malignant glioma cells. Br. J. Cancer 2003, 88, 1277–1280.
  3. Li, J.; Poi, M.J.; Tsai, M.-D. Regulatory mechanisms of tumor suppressor P16(INK4A) and their relevance to cancer. Biochemistry 2011, 50, 5566–5582.
  4. Cilluffo, D.; Barra, V.; Di Leonardo, A. P14ARF: The Absence that Makes the Difference. Genes 2020, 11, 824.
  5. Blanpain, C.; Fuchs, E. Epidermal Stem Cells of the Skin. Annu. Rev. Cell Dev. Biol. 2006, 22, 339–373.
  6. Dimri, G.P.; Lee, X.; Basile, G.; Acosta, M.; Scott, G.; Roskelley, C.; Medrano, E.E.; Linskens, M.; Rubelj, I.; Pereira-Smith, O. A biomarker that identifies senescent human cells in culture and in aging skin in vivo. Proc. Natl. Acad. Sci. USA 1995, 92, 9363–9367.
  7. Kligman, A.M. Perspectives and Problems in Cutaneous Gerontology. J. Investig. Dermatol. 1979, 73, 39–46.
  8. Montagna, W.; Carlisle, K. Structural Changes in Aging Human Skin. J. Investig. Dermatol. 1979, 73, 47–53.
  9. Mimeault, M.; Batra, S.K. Recent advances on skin-resident stem/progenitor cell functions in skin regeneration, aging and cancers and novel anti-aging and cancer therapies. J. Cell. Mol. Med. 2010, 14, 116–134.
  10. Debacq-Chainiaux, F.; Borlon, C.; Pascal, T.; Royer, V.; Eliaers, F.; Ninane, N.; Carrard, G.; Friguet, B.; de Longueville, F.; Boffe, S.; et al. Repeated exposure of human skin fibroblasts to UVB at subcytotoxic level triggers premature senescence through the TGF-β1 signaling pathway. J. Cell Sci. 2005, 118, 743–758.
  11. Lewis, D.A.; Yi, Q.; Travers, J.B.; Spandau, D.F. UVB-induced Senescence in Human Keratinocytes Requires a Functional Insulin-like Growth Factor-1 Receptor and p53. Mol. Biol. Cell 2008, 19, 1346–1353.
  12. McCart, E.A.; Thangapazham, R.L.; Lombardini, E.D.; Mog, S.R.; Panganiban, R.A.M.; Dickson, K.M.; Mansur, R.A.; Nagy, V.; Kim, S.-Y.; Selwyn, R.; et al. Accelerated senescence in skin in a murine model of radiation-induced multi-organ injury. J. Radiat. Res. 2017, 58, 636–646.
  13. Nobori, T.; Miura, K.; Wu, D.J.; Lois, A.; Takabayashi, K.; Carson, D.A. Deletions of the cyclin-dependent kinase-4 inhibitor gene in multiple human cancers. Nature 1994, 368, 753–756.
  14. Scholes, A.G.; Liloglou, T.; Maloney, P.; Hagan, S.; Nunn, J.; Hiscott, P.; Damato, B.E.; Grierson, I.; Field, J.K. Loss of heterozygosity on chromosomes 3, 9, 13, and 17, including the retinoblastoma locus, in uveal melanoma. Investig. Ophthalmol. Vis. Sci. 2001, 42, 2472–2477.
  15. Castellano, M.; Pollock, P.M.; Walters, M.K.; Sparrow, L.E.; Down, L.M.; Gabrielli, B.G.; Parsons, P.G.; Hayward, N.K. CDKN2A/p16 is inactivated in most melanoma cell lines. Cancer Res. 1997, 57, 4868–4875.
  16. Funk, J.O.; Schiller, P.I.; Barrett, M.T.; Wong, D.J.; Kind, P.; Sander, C.A. p16INK4a expression is frequently decreased and associated with 9p21 loss of heterozygosity in sporadic melanoma. J. Cutan. Pathol. 1998, 25, 291–296.
  17. Straume, O.; Sviland, L.; Akslen, L.A. Loss of nuclear p16 protein expression correlates with increased tumor cell proliferation (Ki-67) and poor prognosis in patients with vertical growth phase melanoma. Clin. Cancer Res. Off. J. Am. Assoc. Cancer Res. 2000, 6, 1845–1853.
  18. Mihic-Probst, D.; Mnich, C.D.; Oberholzer, P.A.; Seifert, B.; Sasse, B.; Moch, H.; Dummer, R. p16 expression in primary malignant melanoma is associated with prognosis and lymph node status. Int. J. Cancer 2006, 118, 2262–2268.
  19. Tyagi, E.; Liu, B.; Li, C.; Liu, T.; Rutter, J.; Grossman, D. Loss of p16INK4A stimulates aberrant mitochondrial biogenesis through a CDK4/Rb-independent pathway. Oncotarget 2017, 8, 55848–55862.
  20. Jenkins, N.C.; Liu, T.; Cassidy, P.; Leachman, S.A.; Boucher, K.M.; Goodson, A.G.; Samadashwily, G.; Grossman, D. The p16INK4A tumor suppressor regulates cellular oxidative stress. Oncogene 2011, 30, 265–274.
  21. Al-Khalaf, H.H.; Mohideen, P.; Nallar, S.C.; Kalvakolanu, D.V.; Aboussekhra, A. The cyclin-dependent kinase inhibitor p16INK4a physically interacts with transcription factor Sp1 and cyclin-dependent kinase 4 to transactivate microRNA-141 and microRNA-146b-5p spontaneously and in response to ultraviolet light-induced DNA damage. J. Biol. Chem. 2013, 288, 35511–35525.
  22. Demaria, M.; Ohtani, N.; Youssef, S.A.; Rodier, F.; Toussaint, W.; Mitchell, J.R.; Laberge, R.-M.; Vijg, J.; Van Steeg, H.; Dollé, M.E.T.; et al. An Essential Role for Senescent Cells in Optimal Wound Healing through Secretion of PDGF-AA. Dev. Cell 2014, 31, 722–733.
  23. Jun, J.-I.; Lau, L.F. The matricellular protein CCN1 induces fibroblast senescence and restricts fibrosis in cutaneous wound healing. Nat. Cell Biol. 2010, 12, 676–685.
  24. Natarajan, E.; Omobono, J.D.; Jones, J.C.; Rheinwald, J.G. Co-expression of p16INK4A and laminin 5 by keratinocytes: A wound-healing response coupling hypermotility with growth arrest that goes awry during epithelial neoplastic progression. J. Investig. Dermatol. Symp. Proc. 2005, 10, 72–85.
  25. Pavey, S.; Conroy, S.; Russell, T.; Gabrielli, B. Ultraviolet Radiation Induces p16CDKN2A Expression in Human Skin1. Cancer Res. 1999, 59, 4185–4189.
  26. Adam, R.C.; Fuchs, E. The Yin and Yang of Chromatin Dynamics In Stem Cell Fate Selection. Trends Genet. 2016, 32, 89–100.
  27. Perdigoto, C.N.; Valdes, V.J.; Bardot, E.S.; Ezhkova, E. Epigenetic regulation of epidermal differentiation. Cold Spring Harb. Perspect. Med. 2014, 4, a015263.
  28. Botchkarev, V.A.; Gdula, M.R.; Mardaryev, A.N.; Sharov, A.A.; Fessing, M.Y. Epigenetic regulation of gene expression in keratinocytes. J. Investig. Dermatol. 2012, 132, 2505–2521.
  29. Eckert, R.L.; Adhikary, G.; Rorke, E.A.; Chew, Y.C.; Balasubramanian, S. Polycomb group proteins are key regulators of keratinocyte function. J. Investig. Dermatol. 2011, 131, 295–301.
  30. Avgustinova, A.; Benitah, S.A. Epigenetic control of adult stem cell function. Nat. Rev. Mol. Cell Biol. 2016, 17, 643–658.
  31. Safwan-Zaiter, H.; Wagner, N.; Michiels, J.-F.; Wagner, K.-D. Dynamic Spatiotemporal Expression Pattern of the Senescence-Associated Factor p16Ink4a in Development and Aging. Cells 2022, 11, 541.
  32. Langlands, K.; Down, G.A.; Kealey, T. Id proteins are dynamically expressed in normal epidermis and dysregulated in squamous cell carcinoma. Cancer Res. 2000, 60, 5929–5933.
  33. D’Arcangelo, D.; Tinaburri, L.; Dellambra, E. The Role of p16INK4a Pathway in Human Epidermal Stem Cell Self-Renewal, Aging and Cancer. Int. J. Mol. Sci. 2017, 18, 1591.
  34. Chen, X.; Wang, Z.; Duan, N.; Zhu, G.; Schwarz, E.M.; Xie, C. Osteoblast-Osteoclast Interactions. Connect. Tissue Res. 2018, 59, 99–107.
  35. Jilka, R.L.; O’Brien, C.A. The Role of Osteocytes in Age-Related Bone Loss. Curr. Osteoporos. Rep. 2016, 14, 16–25.
  36. Almeida, M.; Han, L.; Martin-Millan, M.; Plotkin, L.I.; Stewart, S.A.; Roberson, P.K.; Kousteni, S.; O’Brien, C.A.; Bellido, T.; Parfitt, A.M.; et al. Skeletal involution by age-associated oxidative stress and its acceleration by loss of sex steroids. J. Biol. Chem. 2007, 282, 27285–27297.
  37. Glatt, V.; Canalis, E.; Stadmeyer, L.; Bouxsein, M.L. Age-related changes in trabecular architecture differ in female and male C57BL/6J mice. J. Bone Miner. Res. 2007, 22, 1197–1207.
  38. Piemontese, M.; Almeida, M.; Robling, A.G.; Kim, H.-N.; Xiong, J.; Thostenson, J.D.; Weinstein, R.S.; Manolagas, S.C.; O’Brien, C.A.; Jilka, R.L. Old age causes de novo intracortical bone remodeling and porosity in mice. JCI Insight 2017, 2, 93771.
  39. Ucer, S.; Iyer, S.; Kim, H.-N.; Han, L.; Rutlen, C.; Allison, K.; Thostenson, J.D.; de Cabo, R.; Jilka, R.L.; O’Brien, C.; et al. The Effects of Aging and Sex Steroid Deficiency on the Murine Skeleton Are Independent and Mechanistically Distinct. J. Bone Miner. Res. 2017, 32, 560–574.
  40. Marie, P.J. Bone Cell Senescence: Mechanisms and Perspectives. J. Bone Miner. Res. 2014, 29, 1311–1321.
  41. Baron, R.; Kneissel, M. WNT signaling in bone homeostasis and disease: From human mutations to treatments. Nat. Med. 2013, 19, 179–192.
  42. Farr, J.N.; Fraser, D.G.; Wang, H.; Jaehn, K.; Ogrodnik, M.B.; Weivoda, M.M.; Drake, M.T.; Tchkonia, T.; LeBrasseur, N.K.; Kirkland, J.L.; et al. Identification of Senescent Cells in the Bone Microenvironment. J. Bone Miner. Res. 2016, 31, 1920–1929.
  43. Kim, H.-N.; Chang, J.; Shao, L.; Han, L.; Iyer, S.; Manolagas, S.C.; O’Brien, C.A.; Jilka, R.L.; Zhou, D.; Almeida, M. DNA damage and senescence in osteoprogenitors expressing Osx1 may cause their decrease with age. Aging Cell 2017, 16, 693–703.
  44. Farr, J.N.; Xu, M.; Weivoda, M.M.; Monroe, D.G.; Fraser, D.G.; Onken, J.L.; Negley, B.A.; Sfeir, J.G.; Ogrodnik, M.B.; Hachfeld, C.M.; et al. Targeting cellular senescence prevents age-related bone loss in mice. Nat. Med. 2017, 23, 1072–1079.
  45. Kim, H.-N.; Chang, J.; Iyer, S.; Han, L.; Campisi, J.; Manolagas, S.C.; Zhou, D.; Almeida, M. Elimination of senescent osteoclast progenitors has no effect on the age-associated loss of bone mass in mice. Aging Cell 2019, 18, e12923.
  46. Peng, S.; Chen, X.; Huang, C.; Yang, C.; Situ, M.; Zhou, Q.; Ling, Y.; Huang, H.; Huang, M.; Zhang, Y.; et al. UBE2S as a novel ubiquitinated regulator of p16 and β-catenin to promote bone metastasis of prostate cancer. Int. J. Biol. Sci. 2022, 18, 3528–3543.
  47. Harris, A.S.; Thomas, R.G.; Passant, C.D. Do patients with p16-positive oropharyngeal squamous cell carcinoma get more bone metastasis than p16-negative patients? J. Laryngol. Otol. 2018, 132, 429–433.
  48. Righi, A.; Gambarotti, M.; Sbaraglia, M.; Sisto, A.; Ferrari, S.; Dei Tos, A.P.; Picci, P. p16 expression as a prognostic and predictive marker in high-grade localized osteosarcoma of the extremities: An analysis of 357 cases. Hum. Pathol. 2016, 58, 15–23.
  49. Chandra, A.; Lagnado, A.B.; Farr, J.N.; Doolittle, M.; Tchkonia, T.; Kirkland, J.L.; LeBrasseur, N.K.; Robbins, P.D.; Niedernhofer, L.J.; Ikeno, Y.; et al. Targeted clearance of p21- but not p16-positive senescent cells prevents radiation-induced osteoporosis and increased marrow adiposity. Aging Cell 2022, 21, e13602.
  50. Li, J.; Karim, M.A.; Che, H.; Geng, Q.; Miao, D. Deletion of p16 prevents estrogen deficiency-induced osteoporosis by inhibiting oxidative stress and osteocyte senescence. Am. J. Transl. Res. 2020, 12, 672–683.
  51. Ding, Q.; Liu, H.; Liu, L.; Ma, C.; Qin, H.; Wei, Y.; Ren, Y. Deletion of p16 accelerates fracture healing in geriatric mice. Am. J. Transl. Res. 2021, 13, 11107.
  52. Mercado, N.; Ito, K.; Barnes, P.J. Accelerated ageing of the lung in COPD: New concepts. Thorax 2015, 70, 482–489.
  53. Fukuchi, Y. The aging lung and chronic obstructive pulmonary disease: Similarity and difference. Proc. Am. Thorac. Soc. 2009, 6, 570–572.
  54. John-Schuster, G.; Günter, S.; Hager, K.; Conlon, T.M.; Eickelberg, O.; Yildirim, A.Ö. Inflammaging increases susceptibility to cigarette smoke-induced COPD. Oncotarget 2016, 7, 30068–30083.
  55. Meiners, S.; Eickelberg, O.; Königshoff, M. Hallmarks of the ageing lung. Eur. Respir. J. 2015, 45, 807–827.
  56. Selman, M.; Buendía-Roldán, I.; Pardo, A. Aging and Pulmonary Fibrosis. Rev. Investig. Clin. 2016, 68, 75–83.
  57. Venosa, A. Senescence in Pulmonary Fibrosis: Between Aging and Exposure. Front. Med. 2020, 7, 606462.
  58. Kheradmand, F.; You, R.; Hee Gu, B.; Corry, D.B. Cigarette Smoke and DNA Cleavage Promote Lung Inflammation and Emphysema. Trans. Am. Clin. Climatol. Assoc. 2017, 128, 222–233.
  59. Nyunoya, T.; Monick, M.M.; Klingelhutz, A.L.; Glaser, H.; Cagley, J.R.; Brown, C.O.; Matsumoto, E.; Aykin-Burns, N.; Spitz, D.R.; Oshima, J.; et al. Cigarette Smoke Induces Cellular Senescence via Werner’s Syndrome Protein Down-regulation. Am. J. Respir. Crit. Care Med. 2009, 179, 279–287.
  60. Nyunoya, T.; Monick, M.M.; Klingelhutz, A.; Yarovinsky, T.O.; Cagley, J.R.; Hunninghake, G.W. Cigarette Smoke Induces Cellular Senescence. Am. J. Respir. Cell Mol. Biol. 2006, 35, 681–688.
  61. Rashid, K.; Sundar, I.K.; Gerloff, J.; Li, D.; Rahman, I. Lung cellular senescence is independent of aging in a mouse model of COPD/emphysema. Sci. Rep. 2018, 8, 9023.
  62. Cottage, C.T.; Peterson, N.; Kearley, J.; Berlin, A.; Xiong, X.; Huntley, A.; Zhao, W.; Brown, C.; Migneault, A.; Zerrouki, K.; et al. Targeting p16-induced senescence prevents cigarette smoke-induced emphysema by promoting IGF1/Akt1 signaling in mice. Commun. Biol. 2019, 2, 307.
  63. Wang, C.-W.; Wu, T.-I.; Yu, C.-T.; Wu, Y.-C.; Teng, Y.-H.; Chin, S.-Y.; Lai, C.-H.; Chen, T.-C. Usefulness of p16 for differentiating primary pulmonary squamous cell carcinoma from cervical squamous cell carcinoma metastatic to the lung. Am. J. Clin. Pathol. 2009, 131, 715–722.
  64. Belinsky, S.A.; Nikula, K.J.; Palmisano, W.A.; Michels, R.; Saccomanno, G.; Gabrielson, E.; Baylin, S.B.; Herman, J.G. Aberrant methylation of p16(INK4a) is an early event in lung cancer and a potential biomarker for early diagnosis. Proc. Natl. Acad. Sci. USA 1998, 95, 11891–11896.
  65. Okamoto, A.; Hussain, S.P.; Hagiwara, K.; Spillare, E.A.; Rusin, M.R.; Demetrick, D.J.; Serrano, M.; Hannon, G.J.; Shiseki, M.; Zariwala, M.; et al. Mutations in the p16INK4/MTS1/CDKN2, p15INK4B/MTS2, and p18 Genes in Primary and Metastatic Lung Cancer1. Cancer Res. 1995, 55, 1448–1451.
  66. Tong, J.; Sun, X.; Cheng, H.; Zhao, D.; Ma, J.; Zhen, Q.; Cao, Y.; Zhu, H.; Bai, J. Expression of p16 in non-small cell lung cancer and its prognostic significance: A meta-analysis of published literatures. Lung Cancer 2011, 74, 155–163.
  67. p16 Regulation of Lung Epithelial Cell Growth, Repair after Injury and Transformation—ProQuest. Available online: https://www.proquest.com/openview/c4b38b5ea3ce9a758bbacff031039f5c/1?pq-origsite=gscholar&cbl=18750&diss=y (accessed on 28 July 2022).
  68. De Mochel, N.R.; Cheong, K.N.; Cassandras, M.; Wang, C.; Krasilnikov, M.; Matatia, P.; Molofsky, A.; Campisi, J.; Peng, T. Sentinel p16INK4a+ cells in the basement membrane form a reparative niche in the lung 2020. bioRxiv 2020.
  69. Molofsky, A.V.; Slutsky, S.G.; Joseph, N.M.; He, S.; Pardal, R.; Krishnamurthy, J.; Sharpless, N.E.; Morrison, S.J. Increasing p16INK4a expression decreases forebrain progenitors and neurogenesis during ageing. Nature 2006, 443, 448–452.
  70. Song, P.; An, J.; Zou, M.-H. Immune Clearance of Senescent Cells to Combat Ageing and Chronic Diseases. Cells 2020, 9, 671.
  71. Lok, K.; Zhao, H.; Shen, H.; Wang, Z.; Gao, X.; Zhao, W.; Yin, M. Characterization of the APP/PS1 mouse model of Alzheimer’s disease in senescence accelerated background. Neurosci. Lett. 2013, 557, 84–89.
  72. Dorigatti, A.O.; Riordan, R.; Yu, Z.; Ross, G.; Wang, R.; Reynolds-Lallement, N.; Magnusson, K.; Galvan, V.; Perez, V.I. Brain cellular senescence in mouse models of Alzheimer’s disease. GeroScience 2022, 44, 1157–1168.
  73. Musi, N.; Valentine, J.M.; Sickora, K.R.; Baeuerle, E.; Thompson, C.S.; Shen, Q.; Orr, M.E. Tau protein aggregation is associated with cellular senescence in the brain. Aging Cell 2018, 17, e12840.
  74. Ramsden, M.; Kotilinek, L.; Forster, C.; Paulson, J.; McGowan, E.; SantaCruz, K.; Guimaraes, A.; Yue, M.; Lewis, J.; Carlson, G.; et al. Age-Dependent Neurofibrillary Tangle Formation, Neuron Loss, and Memory Impairment in a Mouse Model of Human Tauopathy (P301L). J. Neurosci. 2005, 25, 10637–10647.
  75. Mv, S.; Hv, V. Astrocytes: Biology and pathology. Acta Neuropathol. 2010, 119, 7–35.
  76. Halassa, M.M.; Fellin, T.; Haydon, P.G. Tripartite synapses: Roles for astrocytic purines in the control of synaptic physiology and behavior. Neuropharmacology 2009, 57, 343–346.
  77. Pertusa, M.; García-Matas, S.; Rodriguez-Farre, E.; Sanfeliu, C.; Cristòfol, R. Astrocytes aged in vitro show a decreased neuroprotective capacity. J. Neurochem. 2007, 101, 794–805.
  78. Cohen, J.; Torres, C. Astrocyte senescence: Evidence and significance. Aging Cell 2019, 18, e12937.
  79. Jen, J.; Harper, J.W.; Bigner, S.H.; Bigner, D.D.; Papadopoulos, N.; Markowitz, S.; Willson, J.K.V.; Kinzler, K.W.; Vogelstein, B. Deletion of p16 and p15 Genes in Brain Tumors1. Cancer Res. 1994, 54, 6353–6358.
  80. Ueki, K.; Ono, Y.; Henson, J.W.; Efird, J.T.; von Deimling, A.; Louis, D.N. CDKN2/p16 or RB Alterations Occur in the Majority of Glioblastomas and Are Inversely Correlated1. Cancer Res. 1996, 56, 150–153.
  81. Park, J.W.; Kang, J.; Lim, K.Y.; Kim, H.; Kim, S.-I.; Won, J.K.; Park, C.-K.; Park, S.-H. The prognostic significance of p16 expression pattern in diffuse gliomas. J. Pathol. Transl. Med. 2021, 55, 102–111.
  82. Fueyo, J.; Gomez-Manzano, C.; Puduvalli, V.K.; Martin-Duque, P.; Perez-Soler, R.; Levin, V.A.; Yung, W.K.; Kyritsis, A.P. Adenovirus-mediated p16 transfer to glioma cells induces G1 arrest and protects from paclitaxel and topotecan: Implications for therapy. Int. J. Oncol. 1998, 12, 665–674.
  83. Kranenburg, O.; van der Eb, A.J.; Zantema, A. Cyclin D1 is an essential mediator of apoptotic neuronal cell death. EMBO J. 1996, 15, 46–54.
  84. Kfoury, N.; Sun, T.; Yu, K.; Rockwell, N.; Tinkum, K.L.; Qi, Z.; Warrington, N.M.; McDonald, P.; Roy, A.; Weir, S.J.; et al. Cooperative p16 and p21 action protects female astrocytes from transformation. Acta Neuropathol. Commun. 2018, 6, 12.
  85. Yabluchanskiy, A.; Tarantini, S.; Balasubramanian, P.; Kiss, T.; Csipo, T.; Fülöp, G.A.; Lipecz, A.; Ahire, C.; DelFavero, J.; Nyul-Toth, A.; et al. Pharmacological or genetic depletion of senescent astrocytes prevents whole brain irradiation–induced impairment of neurovascular coupling responses protecting cognitive function in mice. GeroScience 2020, 42, 409–428.
  86. Qian, J.; Wang, X.; Cao, J.; Zhang, W.; Lu, C.; Chen, X. Dihydromyricetin attenuates D-galactose-induced brain aging of mice via inhibiting oxidative stress and neuroinflammation. Neurosci. Lett. 2021, 756, 135963.
  87. Torella, D.; Rota, M.; Nurzynska, D.; Musso, E.; Monsen, A.; Shiraishi, I.; Zias, E.; Walsh, K.; Rosenzweig, A.; Sussman, M.A.; et al. Cardiac stem cell and myocyte aging, heart failure, and insulin-like growth factor-1 overexpression. Circ. Res. 2004, 94, 514–524.
  88. Chimenti, C.; Kajstura, J.; Torella, D.; Urbanek, K.; Heleniak, H.; Colussi, C.; Di Meglio, F.; Nadal-Ginard, B.; Frustaci, A.; Leri, A.; et al. Senescence and Death of Primitive Cells and Myocytes Lead to Premature Cardiac Aging and Heart Failure. Circ. Res. 2003, 93, 604–613.
  89. Anderson, R.; Lagnado, A.; Maggiorani, D.; Walaszczyk, A.; Dookun, E.; Chapman, J.; Birch, J.; Salmonowicz, H.; Ogrodnik, M.; Jurk, D.; et al. Length-independent telomere damage drives post-mitotic cardiomyocyte senescence. EMBO J. 2019, 38, e100492.
  90. Lewis-McDougall, F.C.; Ruchaya, P.J.; Domenjo-Vila, E.; Shin Teoh, T.; Prata, L.; Cottle, B.J.; Clark, J.E.; Punjabi, P.P.; Awad, W.; Torella, D.; et al. Aged-senescent cells contribute to impaired heart regeneration. Aging Cell 2019, 18, e12931.
  91. Kajstura, J.; Pertoldi, B.; Leri, A.; Beltrami, C.-A.; Deptala, A.; Darzynkiewicz, Z.; Anversa, P. Telomere Shortening Is an in Vivo Marker of Myocyte Replication and Aging. Am. J. Pathol. 2000, 156, 813–819.
  92. Matthews, C.; Gorenne, I.; Scott, S.; Figg, N.; Kirkpatrick, P.; Ritchie, A.; Goddard, M.; Bennett, M. Vascular Smooth Muscle Cells Undergo Telomere-Based Senescence in Human Atherosclerosis. Circ. Res. 2006, 99, 156–164.
  93. Cianflone, E.; Torella, M.; Biamonte, F.; De Angelis, A.; Urbanek, K.; Costanzo, F.S.; Rota, M.; Ellison-Hughes, G.M.; Torella, D. Targeting Cardiac Stem Cell Senescence to Treat Cardiac Aging and Disease. Cells 2020, 9, 1558.
  94. Epstein, J.A. A Time to Press Reset and Regenerate Cardiac Stem Cell Biology. JAMA Cardiol. 2019, 4, 95–96.
  95. Baker, D.J.; Childs, B.G.; Durik, M.; Wijers, M.E.; Sieben, C.J.; Zhong, J.; Saltness, R.A.; Jeganathan, K.B.; Verzosa, G.C.; Pezeshki, A.; et al. Naturally occurring p16(Ink4a)-positive cells shorten healthy lifespan. Nature 2016, 530, 184–189.
  96. Grosse, L.; Wagner, N.; Emelyanov, A.; Molina, C.; Lacas-Gervais, S.; Wagner, K.-D.; Bulavin, D.V. Defined p16High Senescent Cell Types Are Indispensable for Mouse Healthspan. Cell Metab. 2020, 32, 87–99e6.
  97. Shi, J.; Sun, J.; Liu, L.; Shan, T.; Meng, H.; Yang, T.; Wang, S.; Wei, T.; Chen, B.; Ma, Y.; et al. P16ink4a overexpression ameliorates cardiac remodeling of mouse following myocardial infarction via CDK4/pRb pathway. Biochem. Biophys. Res. Commun. 2022, 595, 62–68.
  98. Joosten, S.A.; van Ham, V.; Nolan, C.E.; Borrias, M.C.; Jardine, A.G.; Shiels, P.G.; van Kooten, C.; Paul, L.C. Telomere Shortening and Cellular Senescence in a Model of Chronic Renal Allograft Rejection. Am. J. Pathol. 2003, 162, 1305–1312.
  99. Chkhotua, A.B.; Gabusi, E.; Altimari, A.; D’Errico, A.; Yakubovich, M.; Vienken, J.; Stefoni, S.; Chieco, P.; Yussim, A.; Grigioni, W.F. Increased expression of p16(INK4a) and p27(Kip1) cyclin-dependent kinase inhibitor genes in aging human kidney and chronic allograft nephropathy. Am. J. Kidney Dis. 2003, 41, 1303–1313.
  100. Melk, A.; Schmidt, B.M.W.; Vongwiwatana, A.; Rayner, D.C.; Halloran, P.F. Increased Expression of Senescence-Associated Cell Cycle Inhibitor p16INK4a in Deteriorating Renal Transplants and Diseased Native Kidney. Am. J. Transplant. 2005, 5, 1375–1382.
  101. Melk, A.; Schmidt, B.M.W.; Takeuchi, O.; Sawitzki, B.; Rayner, D.C.; Halloran, P.F. Expression of p16INK4a and other cell cycle regulator and senescence associated genes in aging human kidney. Kidney Int. 2004, 65, 510–520.
  102. Sis, B.; Tasanarong, A.; Khoshjou, F.; Dadras, F.; Solez, K.; Halloran, P.F. Accelerated expression of senescence associated cell cycle inhibitor p16INK4A in kidneys with glomerular disease. Kidney Int. 2007, 71, 218–226.
  103. Westhoff, J.H.; Hilgers, K.F.; Steinbach, M.P.; Hartner, A.; Klanke, B.; Amann, K.; Melk, A. Hypertension induces somatic cellular senescence in rats and humans by induction of cell cycle inhibitor p16INK4a. Hypertension 2008, 52, 123–129.
  104. Liu, J.; Yang, J.-R.; Chen, X.-M.; Cai, G.-Y.; Lin, L.-R.; He, Y.-N. Impact of ER stress-regulated ATF4/p16 signaling on the premature senescence of renal tubular epithelial cells in diabetic nephropathy. Am. J. Physiol.-Cell Physiol. 2015, 308, C621–C630.
  105. Gu, X.; Peng, C.-Y.; Lin, S.-Y.; Qin, Z.-Y.; Liang, J.-L.; Chen, H.-J.; Hou, C.-X.; Wang, R.; Du, Y.-Q.; Jin, J.-L.; et al. P16INK4a played a critical role in exacerbating acute tubular necrosis in acute kidney injury. Am. J. Transl. Res. 2019, 11, 3850–3861.
  106. Jin, J.; Tao, J.; Gu, X.; Yu, Z.; Wang, R.; Zuo, G.; Li, Q.; Lv, X.; Miao, D. P16 INK4a Deletion Ameliorated Renal Tubulointerstitial Injury in a Stress-induced Premature Senescence Model of Bmi-1 Deficiency. Sci. Rep. 2017, 7, 7502.
  107. Baiocchi, L.; Glaser, S.; Francis, H.; Kennedy, L.; Felli, E.; Alpini, G.; Gracia-Sancho, J. Impact of Aging on Liver Cells and Liver Disease: Focus on the Biliary and Vascular Compartments. Hepatol. Commun. 2021, 5, 1125–1137.
  108. Kim, H.; Kisseleva, T.; Brenner, D.A. Aging and liver disease. Curr. Opin. Gastroenterol. 2015, 31, 184–191.
  109. Aravinthan, A.D.; Alexander, G.J.M. Senescence in chronic liver disease: Is the future in aging? J. Hepatol. 2016, 65, 825–834.
  110. Zhu, C.; Ikemoto, T.; Utsunomiya, T.; Yamada, S.; Morine, Y.; Imura, S.; Arakawa, Y.; Takasu, C.; Ishikawa, D.; Shimada, M. Senescence-related genes possibly responsible for poor liver regeneration after hepatectomy in elderly patients. J. Gastroenterol. Hepatol. 2014, 29, 1102–1108.
  111. Sawada, N. Hepatocytes from old rats retain responsiveness of c-myc expression to EGF in primary culture but do not enter S phase. Exp. Cell Res. 1989, 181, 584–588.
  112. Maeso-Díaz, R.; Ortega-Ribera, M.; Fernández-Iglesias, A.; Hide, D.; Muñoz, L.; Hessheimer, A.J.; Vila, S.; Francés, R.; Fondevila, C.; Albillos, A.; et al. Effects of aging on liver microcirculatory function and sinusoidal phenotype. Aging Cell 2018, 17, e12829.
  113. Omori, S.; Wang, T.-W.; Johmura, Y.; Kanai, T.; Nakano, Y.; Kido, T.; Susaki, E.A.; Nakajima, T.; Shichino, S.; Ueha, S.; et al. Generation of a p16 Reporter Mouse and Its Use to Characterize and Target p16high Cells In Vivo. Cell Metab. 2020, 32, 814–828e6.
  114. González-Navarro, H.; Vinué, Á.; Sanz, M.J.; Delgado, M.; Pozo, M.A.; Serrano, M.; Burks, D.J.; Andrés, V. Increased dosage of Ink4/Arf protects against glucose intolerance and insulin resistance associated with aging. Aging Cell 2013, 12, 102–111.
  115. Pal, A.; Potjer, T.P.; Thomsen, S.K.; Ng, H.J.; Barrett, A.; Scharfmann, R.; James, T.J.; Bishop, D.T.; Karpe, F.; Godsland, I.F.; et al. Loss-of-Function Mutations in the Cell-Cycle Control Gene CDKN2A Impact on Glucose Homeostasis in Humans. Diabetes 2016, 65, 527–533.
  116. Bantubungi, K.; Hannou, S.-A.; Caron-Houde, S.; Vallez, E.; Baron, M.; Lucas, A.; Bouchaert, E.; Paumelle, R.; Tailleux, A.; Staels, B. Cdkn2a/p16Ink4a regulates fasting-induced hepatic gluconeogenesis through the PKA-CREB-PGC1α pathway. Diabetes 2014, 63, 3199–3209.
  117. Deleye, Y.; Cotte, A.K.; Hannou, S.A.; Hennuyer, N.; Bernard, L.; Derudas, B.; Caron, S.; Legry, V.; Vallez, E.; Dorchies, E.; et al. CDKN2A/p16INK4a suppresses hepatic fatty acid oxidation through the AMPKα2-SIRT1-PPARα signaling pathway. J. Biol. Chem. 2020, 295, 17310–17322.
  118. Ogrodnik, M.; Miwa, S.; Tchkonia, T.; Tiniakos, D.; Wilson, C.L.; Lahat, A.; Day, C.P.; Burt, A.; Palmer, A.; Anstee, Q.M.; et al. Cellular senescence drives age-dependent hepatic steatosis. Nat. Commun. 2017, 8, 15691.
  119. Zhang, X.; Xu, G.B.; Zhou, D.; Pan, Y.-X. High-fat diet modifies expression of hepatic cellular senescence gene p16(INK4a) through chromatin modifications in adult male rats. Genes Nutr. 2018, 13, 6.
  120. Zang, J.-J.; Xie, F.; Xu, J.-F.; Qin, Y.-Y.; Shen, R.-X.; Yang, J.-M.; He, J. P16 gene hypermethylation and hepatocellular carcinoma: A systematic review and meta-analysis. World J. Gastroenterol. 2011, 17, 3043–3048.
  121. Wong, I.H.N.; Dennis Lo, Y.M.; Zhang, J.; Liew, C.-T.; Ng, M.H.L.; Wong, N.; Lai, P.B.S.; Lau, W.Y.; Hjelm, N.M.; Johnson, P.J. Detection of Aberrant p16 Methylation in the Plasma and Serum of Liver Cancer Patients1. Cancer Res. 1999, 59, 71–73.
More
© Text is available under the terms and conditions of the Creative Commons Attribution (CC BY) license (http://creativecommons.org/licenses/by/4.0/)
ScholarVision Creations
Feedback