• Log in with Facebook Log in with Twitter Log In with Google      Sign In    
  • Create Account
              Advocacy & Research for Unlimited Lifespans


Cell senescence contributes to tissue regeneration in zebrafish

cellular senescence regeneration tissue injury zebrafish

  • Please log in to reply
No replies to this topic
⌛⇒ MITOMOUSE has been fully funded!

#1 Engadin

  • Guest
  • 116 posts
  • 272
  • Location:Madrid
  • NO

Posted 05 November 2019 - 07:44 PM





F U L L   T E X T   S O U R C E :   Aging Cell






Cellular senescence is a stress response that limits the proliferation of damaged cells by establishing a permanent cell cycle arrest. Different stimuli can trigger senescence but excessive production or impaired clearance of these cells can lead to their accumulation during aging with deleterious effects. Despite this potential negative side of cell senescence, its physiological role as a pro‐regenerative and morphogenetic force has emerged recently after the identification of programmed cell senescence during embryogenesis and during wound healing and limb regeneration. Here, we explored the conservation of tissue injury‐induced senescence in a model of complex regeneration, the zebrafish. Fin amputation in adult fish led to the appearance of senescent cells at the site of damage, and their removal impaired tissue regeneration. Despite many conceptual similarities, this tissue repair response is different from developmental senescence. Our results lend support to the notion that cell senescence is a positive response promoting tissue repair and homeostasis.
Cellular senescence is a terminal cell response consisting on the implementation of a permanent cell cycle arrest and the acquisition of a secretory phenotype with cell‐to‐cell communication properties (Collado, Blasco, & Serrano, 2007; Muñoz‐Espín & Serrano, 2014). Exhaustion of the proliferative capacity of the cell leads to senescence, and the accumulation of these damaged cells in tissues from old individuals is considered a key element in the process of aging (van Deursen, 2014). Despite this detrimental effect, the senescence response has a beneficial side protecting damaged cells from proliferating. This is considered the basis of its tumor‐suppressive function (Collado et al., 2007; Collado & Serrano, 2010). The recent identification of developmentally programmed cell senescence during embryogenesis expanded our view of the positive activities of this response (Muñoz‐Espín et al., 2013; Storer et al., 2013). Senescence during development promotes cell turnover, tissue remodeling, and, paradoxically, growth. A similar positive pro‐morphogenetic activity for cell senescence has been suggested to operate during skin wound healing in mice (Demaria et al., 2014) and during limb regeneration in salamanders (Yun, Davaapil, & Brockes, 2015). Senescent cells seem to appear at wound sites after injury to help promote optimal wound healing (Yun, 2018).
Here, we decided to evaluate the senescence response in the context of tissue injury using an animal model of complex tissue regeneration, the zebrafish. To study senescence after tissue damage, we amputated the pectoral fin of adult fish (around 1 year old) at approximately 50% of its length and followed regeneration with time (Figure 1a). We stained fins for senescence‐associated beta‐galactosidase (SAbetaGal), the most widely used marker of senescence (Dimri et al., 1995), after 8, 16, or 30 days postamputation (dpa), a time point in which fins were completely regenerated. Control stainings were performed on the contralateral unamputated fin or immediately after amputation to discard artifacts derived from unspecific staining of damaged tissue. Fins at 8 dpa showed intense blue staining compared with light blue at 16 dpa and completely absent staining at 30 dpa (Figure 1b). Immunohistochemical co‐staining with phospho‐histone 3 (P‐H3), a marker of proliferation, at 8 dpa confirmed that the SAbetaGal‐positive cells were not proliferating (Figure 1b). To further confirm these results, we used an alternative senescence detection method more amenable for quantification, utilizing Galacton, a chemiluminescent substrate (Bassaneze, Miyakawa, & Krieger, 2008). We collected amputated and nonamputated fins at different times during regeneration and split the amputated fins into proximal (closer to the body) and distal (the regenerated area) parts (Figure 1c). Again, we observed that 8 dpa was the time point that produced a stronger SAbetaGal reaction and this activity was restricted to the distal part of the fin, the area where regeneration takes place (Figure 1d). In contrast, the proximal area of the 8 dpa fin and the distal or proximal areas of 16 and 30 dpa fins were mostly negative (Figure 1d).
Figure 1
Pectoral fin amputation induces features of cell senescence. (a) Schematic representation of the fin amputation system used throughout the study. (b) Representative photomicrographs of fins stained for SAbetaGal or phospho‐histone 3 (P‐H3, right panel) after amputations (NA: nonamputated; 8, 16, and 30 dpa: days postamputation). Co‐staining of P‐H3 was done at 8 dpa. Arrowhead shows the amputation plane. © Schematic representation showing the different types of samples used in the study (NA: nonamputated; A: amputated; DIS: distal area; PROX: proximal). (d) SAbetaGal activity measured using Galacton substrate after 8, 16, and 30 days postamputation (dpa) (from 5–10 animals per condition). (e) Expression levels by QPCR of cdkn1a (left panel) and cdkn2ab (right panel) genes relative to the housekeeping gene rps11 after 8, 16, and 30 days postamputation (dpa). Results are presented as mean ± SD ***p < .001, **p < .01,*p < .05, n.s. nonsignificant



We also extracted RNA from amputated distal and proximal fins and unamputated fins, to check for the expression of some genes that have been linked to the induction of senescence in different species (Collado & Serrano, 2006; Hernandez‐Segura, Nehme, & Demaria, 2018) and in zebrafish (Donnini et al., 2010; Xia et al., 2014). Similar to our results with the SAbetaGal detection, the distal part of 8 dpa fins showed higher expression levels of cdkn1a and cdkn2ab than the proximal part of amputated fins or the unamputated contralateral fin (Figure 1e). The expression of these senescence markers returned to normal levels after 16 and 30 dpa, in line with our observations using SAbetaGal.
In summary, these results support the notion of a transient induction of cell senescence during fin regeneration as judged by increased SAbetaGal activity and upregulation of the expression of key senescence genes such as cdkn1a and cdkn2ab. A similar transient induction of senescence has been previously reported during zebrafish heart injury and regeneration (Bednarek et al., 2015).
Triggering senescence after tissue injury could have positive or negative effects on the regenerative capacity of the damaged tissue, due to its potential pro‐regenerative and anti‐proliferative activities, respectively (He & Sharpless, 2017). To directly assess the role of senescence induction during fin amputation, we decided to induce the removal of these senescent cells from amputated fins. For this, we treated fish for 48 or 72 hr with ABT‐263 (Navitoclax), a senolytic compound that by inhibiting the Bcl‐2 antiapoptotic family of proteins triggers specifically the death of the senescent cells (Chang et al., 2016). We determined the activity of the SAbetaGal enzyme in extracts from unamputated fins as control and from the proximal and distal regions of amputated fins that were previously treated with ABT‐263 for 48 or 72 hr or that were incubated with vehicle as a negative control (Figure 2a). ABT‐263 treatment caused a reduction in SAbetaGal staining and a concomitant induction of apoptosis in the regenerating area, as determined by TUNEL staining (Figure S1A–C). We quantified SAbetaGal activity at 8 dpa, the day at which we had observed the peak of senescence induction. We confirmed the induction of SAbetaGal activity in the vehicle‐treated fish and observed that the activity present in the extracts from the regenerating (distal) region was blunted by the ABT‐263 treatment (Figure 2b). Furthermore, mRNA expression analysis of cdkn1a and cdkn2ab after ABT‐263 treatment also confirmed the drastic reduction in the levels of these senescence markers at the regenerating area after 48 and 72 hr of incubation (Figure 2c).
Figure 2
Removal of senescent cells impairs fin regeneration. (a) Schematic representation of the experimental strategy followed to analyze the effect of removing senescent cells from amputated fins after incubation with ABT‐263 for 48 or 72 hr, or treated with vehicle (VEH). (b) SAbetaGal activity measured using Galacton substrate at 8 days postamputation and after treatment with ABT‐263 for 48 or 72 hr, or with vehicle (VEH) (from 5–10 animals per condition). © Expression levels by QPCR of cdkn1a (left panel) and cdkn2ab (right panel) genes relative to the housekeeping gene rps11 at 8 dpa and after treatment with ABT‐263 for 48 or 72 hr, or with vehicle (VEH). (d) Length of regenerate (%) reached by amputated fins at 8 days postamputation and after treatment with ABT‐263 relative to untreated amputated fins (five animals per group). (e) Representative photomicrographs of larval fins stained for SAbetaGal or p21, 24 hr after amputation and control fin (CTRL). Scale bars: SAbetaGAL: 200 µm; p21: 75 µm. Results are presented as mean ± SD ***p < .001, **p < .01, *p < .05, n.s. nonsignificant.

Also tagged with one or more of these keywords: cellular senescence, regeneration, tissue injury, zebrafish

1 user(s) are reading this topic

0 members, 1 guests, 0 anonymous users