- Academic Editor
Background: Exposure to low dose rate (LDR) radiation may accelerate
aging processes. Previously, we identified numerous LDR-induced pathways involved
in oxidative stress (OS) and antioxidant systems, suggesting that these pathways
protect against premature senescence (PS). This study aimed to investigate if
there are differences between young replicative senescent (RS) and PS cells
considering DNA repair kinetics, OS, and DNA damage localized in the telomeres.
Methods: We established PS cells by culturing and passaging young
primary fibroblasts exposed to LDR. Then, RS cells were established by culturing
and passaging young fibroblasts until they stopped proliferating. Senescence was
characterized by analyzing telomere length and senescence-associated
Cellular senescence is involved in organism aging and tumor control, and substantial progress has been made in defining the mechanisms involved [1, 2]. There is also a significant amount of experimental data suggesting that endogenous, as well as exogenous production of reactive oxygen species (ROS)—for example from exposure to acute ionizing radiation—contributes to senescence [3]; however, there is limited knowledge about the mechanism of premature senescence (PS) induced by chronic irradiation.
Senescence, as defined by Hayflick and Moorhead, occurs when cells remain viable
but lose proliferative capability irreversibly after being cultured for a period
of time [4], signifying that normal human diploid cells have a finite number of
population doublings. The characteristics of senescent cells include growth
arrest, expression of lysosomal beta-galactosidase (SA-
Progress has been made in defining the mechanisms that contribute to senescence
[1, 2, 18], including the involvement of ROS and DNA damage [3]. It was shown
that growth arrest at the G1 phase is initiated by DNA damage that signals the
upregulation of CDKN1A/p21
In the present investigation, we used human diploid primary fibroblasts VH10
cells which was a gift from Prof. Leon Mullenders, Department of Radiation
Genetics and Chemical Mutagenesis, Leiden Medical University, the Netherlands.
Different passages of VH10 cells were cultured in 12 mL of Dulbecco’s modified
minimum essential medium (Sigma-Aldrich, Darmstadt, Germany) supplemented with
10% bovine serum (Sigma-Aldrich) and 1%
penicillin-streptomycin (Sigma-Aldrich). The cells were validated and tested
negative for mycoplasma. The cells were cultured in a humidified cell culture
incubator at 37 °C and 5% CO
PD = ln (N
Further, the growth rate kinetics for the cells were established based on the
accumulated number of population doublings each week. According to our previous
results [32], we divided cells into three groups based on their senescence
status: (1) “young cells” with passage number 13 or less (long telomere length
(T/S ratio of 1), low SA-
To establish the growth rate kinetics under chronic irradiation, a cell culture
incubator equipped with a custom-made
The experimental design for establishing premature senescent cells: P19-C, non-irradiated control; P19-ST, 6 weeks chronically irradiated P13 cells with 2 weeks recovery time; and P19-IR, 6 weeks chronically irradiated P13 cells with a further 2 weeks incubation under chronic irradiation.
To establish DNA repair kinetics, young, middle-aged, and senescent cells were
irradiated acutely with 1 Gy at a dose rate of 0.75 Gy/min using
GammaCell
The DNA repair kinetics of the young, premature senescent, and senescent cells
were established using
Cells were prepared for Western blot analysis using our previously published protocol [34]. Briefly, the cells were lysed in Laemmli buffer with proteinase inhibitor (Roche Diagnostics GmbH, Mannheim, Germany). After quantification of protein in the lysates with Protein Assay Reagent (Thermo Scientific, Rockford, IL, USA), 10 µg protein per sample was loaded in a NuPAGE 4–12% Bis–Tris gel (Invitrogen, Waltham, MA, USA) for electrophoresis. The proteins were then transferred from the gel onto a Nitrocellulose membrane (Thermo Scientific) overnight at 30 V (4 °C) using XCell SureLock™ Mini-Cell System (Invitrogen, Waltham, Massachusetts, United States).
The unspecific binding sites on the membrane were then blocked by incubating the membrane in LI-COR blocking buffer (LI-COR, Cambridge, UK) for 90 min. The membrane was washed three times with Tris-buffered saline containing 0.05% Tween (TBST). Following the washing steps, the membrane was incubated with primary antibodies overnight at 4 °C followed by washing steps and secondary antibody incubation (anti-mouse conjugated with IRDye® Infrared Dyes (LI-COR)) before detection of the secondary antibody signals with Odyssey imaging system and quantification of protein bands with Image Studio version 5.2 software (LI-COR, Cambridge, Milton, Cambridge CB4 0WS, United Kingdom). The primary antibodies used were as follows: HO1 (1:1000, from rabbit, Novusbio, Centennial, CO, USA); P21 (1:1000, from mouse, Cell Signaling Technology, Inc., Danvers, MA, USA); hMTH1 (1:1000, from rabbit, Novusbio, Centennial, CO, USA ); and GAPDH (1:10,000, from mouse, Sigma, Saint Louis, MO, USA).
To investigate if
The cells were dehydrated by incubating the slides for 3 min in 70%, followed by 90% and finally 99% ethanol (Absolut finsprit, Malmö, Sweden)/water solutions. The slides were then kept at room temperature for 20 min. The telomere probe, PNA, was prepared in a hybridization solution provided by the company (Alexa 647-OO-ccctaaccctaaccctaa, Panagene, South Korea) at a concentration of 200 nM. The solution was then heated to 90 °C for 5 min and applied on slides, which were then incubated first at 85 °C for 10 min and then overnight at 37 °C in a humidified chamber. Following overnight incubation, the slides were washed two times with a washing solution containing 70% formamide (Sigma-Aldrich) and 10 mM Tris-HCl at pH 7.5, and three times with a washing solution containing 50 mM Tris-HCL (Sigma-Aldrich) pH 7.5, 150 mM NaCl (Sigma-Aldrich), and 0.8% Tween-20.
The nuclei were stained with DAPI for 10 min. The coverslips were then quickly
rinsed with MilliQ water and dehydrated by increasing concentrations of ethanol
as described above. The dried coverslips were mounted with Vectashield and sealed
with nail polish. The slides were stored at 4 °C until imaging with a
microscope was performed. The imaging was performed using a Zeiss LSM 800 (Zeiss
Group, Oberkochen, Baden-Württemberg, Germany) microscope equipped with an AiryScan detector
and a laser for AlexaFluor-647 (Panagene, South Korea). The detector gain was set
to 800–950 V and the digital gain to 1 in super-resolution mode. The signals of
AlexaFluor-647 from the labeled telomeres were captured with 4% excitation power
of a 650 nm laser, and five images (z-stacks, confocal) were captured in
unidirectional frame scanning mode with 2048
SA-
Genomic DNA was extracted from cells at different passages using the
DNeasy® Blood & Tissue kit (Qiagen, Hilden, Germany). The relative telomere length was determined based on a previously described
method [37] with some minor modifications. Briefly, 40 ng DNA was mixed with 2
µL of 5
For the calculation of telomere length, the ratio of telomere length versus the
single standard gene expression (T/S) based on the 2
For the detection of 8-oxo-dG in the medium, a modified competitive enzyme-linked immunosorbent assay (ELISA) method was applied. The method was set up and described by us previously [38, 39]. Firstly, the samples were pre-purified using a Bond Elute column to remove compounds that can cross-react with the primary antibody used in the ELISA method. The pre-purification step was performed two times. For the detection of 8-oxo-dG, 1 mL medium was used and processed following the protocol provided by the company Health Biomarkers Sweden AB, Stockholm, Sweden. All samples were analyzed in triplicate and the concentration of 8-oxo-dG was calculated based on a standard curve covering concentration ranges of 8-oxo-dG from 0.05 to 10 ng/mL. The concentration of 8-oxo-dG was expressed as ng per one million cells.
For each endpoint studied, at least three independent experiments were performed. The Student’s t-test was used to determine the p-values to compare results for irradiated and un-irradiated cells. Plotted results represent the average of experiments and bars correspond to standard error or standard deviation (indicated in the figure legends). A p-value lower than 0.05 was chosen to indicate a significant difference. The effect and interaction of the three factors—weeks in culture, exposure (to 12 mGy/h and no exposure), and the age (P8 and P13) on population doubling and 8-oxo-dG—were investigated by three-way ANOVA statistical analysis with Tukey post-hoc test. The analysis was performed on the data sets to examine which of the three factors show an effect and between which factors interaction can be observed.
The number of population doublings (PDs) of the P8 control cells (Fig. 2A) was
about 2.5
Pupulation doublings of P8 and P13 cells under chronic exposure
to 12 mGy/h. (A) Young cells, passage 8 (P8); and (B) middle-aged cells, passage
13 (P13) with
(
In order to compare the oxidative stress response between P8 and P13 cells, the
cells were exposed to a chronic low dose rate of ionizing radiation for 8 weeks
as described in the materials and methods. Then, the weekly levels of 8-oxo-dG in
the cell culture media from irradiated and non-irradiated cells were analyzed.
The slopes of the curves shown in Fig. 3A were calculated using linear regression
as estimates of average increments of 8-oxo-dG per million cells and week. This
comparison showed that the irradiated P13 cells produced significantly
(p = 0.035) larger amounts of 8-oxo-dG compared to the irradiated P8
cells (on average 27
Oxidatve stress levels of the young, middle aged and senescent
cells. Radiation induced extracellular 8-oxo-dG in the P8 and P13 cells (A) and
the levels and the expressions of (B) HO1 and (C) hMTH1 proteins in the different
passages of the cells used in the study. The solid lines in Fig. 3A are
non-irradiated control cells, and the dash lines are cells exposed at 12
mGy/h. The values are presented as mean
Additionally, we analyzed the expression of 2 proteins involved in oxidative stress, HO1, and hMTH1. The results are summarised in Fig. 3B,C. The results on HO1 (Fig. 3B) indicate no differences in the expression of HO1 among P19-C, P19 IR, P19 ST, and P23. However, compared with P8, a generally lower expression of HO1 was found in P19-C, P19-ST, P19-IR, and P23. The results in Fig. 3C, indicate a slightly, p = 0.09, decreased level of hMTH1 expression in non-irradiated P19-C compared to P8 cells. The expressions were increased in the exposed P19-ST and P19-IR cells as compared with P19-C. The levels of hMTH1 were similar in P8, P19-IR and P23.
The 6-week chronically irradiated P13 (P19-ST, P19-IR, and control
non-irradiated P19-C cells), as well as RS (P23) and young cells (P8) were
prepared for telomere length quantification, SA-
The levels of senescent cells in different passages of VH10
cells analyzed by different methods. (A) T/S ratio analysis by real-time PCR.
The telomere length of P8 cells (the longest) was used as a reference to
normalize the telomere lengths of the replicative and premature senescence cells,
P23 and P19, respectively. (B) The percentage of SA-
The results of SA-
The results are summarized in Fig. 5A,B. The results presented in Fig. 5A show
that P8 VH10 cells have low steady-state levels of
DNA repair kinetics of the young, premature
senescence (PS) and replicative senescent (RS) cells exposed to 1
Gy. (A,B) DNA repair kinetics based on the
DNA DSB repair kinetics were also established for the PS cells, LDR-irradiated
P19-ST and P19-IR, and their non-irradiated control cells, P19-C. The results are
presented in Fig. 5B. Comparing the formation and repair of DSBs between the P19
cell types, no significant differences were observed. However, all the P19 cells
had slightly elevated
Next, we wanted to investigate if the elevated
Telomeric DNA damage and nucleaus size of the young, PS
and RS cells. (A) The levels of telomere dysfunction-induced foci (TIFs) in
young, premature senescent, and replicative senescent cells, in the
LDR-irradiated control cells (cell exposed to LDR but not to 1 Gy acute) and in
the LDR-irradiated cells exposed to 1 Gy, 48 h after the exposure, nc
indicates a p-value
By measuring the diameter of
Sample | Average |
Sample | Average | p values | |
P8 Control | 1.91 |
VS | P8 1 Gy 48 h | 3.88 |
p |
P8 Control | 1.91 |
VS | P19-C Control | 7.95 |
p |
P8 Control | 1.91 |
VS | P19-IR Control | 12.32 |
p |
P8 Control | 1.91 |
VS | P19-ST Control | 11.55 |
p |
P8 Control | 1.91 |
VS | P23 Control | 18.27 |
p |
P8 1 Gy 48 h | 3.88 |
VS | P19-C 1 Gy 48 h | 10.71 |
p |
P8 1 Gy 48 h | 3.88 |
VS | P19-IR 1 Gy 48 h | 14.75 |
p |
P8 1 Gy 48 h | 3.88 |
VS | P19-ST 1 Gy 48 h | 16.33 |
p |
P8 1 Gy 48 h | 3.88 |
VS | P23 1 Gy 48 h | 28.55 |
p |
P19-C Control | 7.95 |
VS | P19-C 1 Gy 48 h | 10.71 |
nc (p = 0.09) |
P19-C Control | 7.95 |
VS | P19-IR Control | 12.32 |
p |
P19-C Control | 7.95 |
VS | P19-ST Control | 11.55 |
p |
P19-C Control | 7.95 |
VS | P23 Control | 18.27 |
p |
P19-C 1 Gy 48 h | 10.71 |
VS | P19-IR 1 Gy 48 h | 14.75 |
nc ( p = 0.08) |
P19-C 1 Gy 48 h | 10.71 |
VS | P19-ST 1 Gy 48 h | 16.33 |
p |
P19-C 1 Gy 48 h | 10.71 |
VS | P23 1 Gy 48 h | 28.55 |
p |
P19-IR Control | 12.32 |
VS | P19-IR 1 Gy 48 h | 14.75 |
nc (p = 0.16) |
P19-IR Control | 12.32 |
VS | P19-ST Control | 11.55 |
nc (p = 0.35) |
P19-IR Control | 12.32 |
VS | P23 Control | 18.27 |
p |
P19-IR 1 Gy 48 h | 14.75 |
VS | P19-ST 1 Gy 48 h | 16.33 |
nc (p = 0.03) |
P19-IR 1 Gy 48 h | 14.75 |
VS | P23 1 Gy 48 h | 28.55 |
p |
P19-ST Control | 11.55 |
VS | P19-ST 1 Gy 48 h | 16.33 |
p |
P19-ST Control | 11.55 |
VS | P23 Control | 18.03 |
p |
P19-ST 1 Gy 48 h | 16.33 |
VS | P23 1 Gy 48 h | 28.55 |
p |
nc, no significant change; TIF, telomere dysfunction-induced γH2AX foci.
P19-IR control and P19-ST control were exposed only to LDR.
We also observed that the size of the nuclei was changed by the age of the
cells. The data in Fig. 6D showed the average size of the nuclei in the cells.
The results are presented as pixel areas of DNA stained by DAPI and indicate a
significantly larger nucleus in the senescent cells than in the young P8 cells
(p
Accumulation of senescent cells is thought to be involved in tissue aging [43]. Cellular senescence is characterized by a permanent cell cycle arrest in parallel with specific metabolic, morphological, and transcriptional changes. Although loss of cell proliferation is limiting the viability of organs and tissues, the senescent cell is still functional and can sustain organ function for a significant length of time. This is a remarkable mechanism of evolution that balances the fate of the biological clock and leads to the optimization of the life span of organs to benefit the organism. However, conditions that induce premature senescence will inevitably shorten the viability of tissues and organs, and could shorten the life span of the organism [44]. The literature also reports on a variety of other beneficial effects of senescent cells, e.g., they contribute to wound-healing [45], improve insulin secretion and delay diabetes [46], exert tumor suppressive activity both by proliferation arrest and by activating immune response [47, 48] and contribute to embryonic development [49].
The majority of results on studies related to radiation-induced senescence are based on radiotherapy using high doses and high dose rates where a significant amount of DNA damage is produced within a short time leading to activation of the DNA damage response, permanent cell cycle arrest/senescence and/or apoptosis [50, 51]. Notably, studies investigating the effects of chronic LDR exposure on cellular and organism aging are few and thus interesting to explore. In the current study, we used a cell culture incubator with a cesium source with low activity placed below the incubator, capable of delivering different dose rates by shielding and adjusting the distance from the source in the incubator where the cells are cultured. In the present experimental design, the cells received a constant 12 mGy/h during growth, taking about 83 h to deliver 1 Gy to cells. One Gy leads to approximately 40 DSBs. At 12 mGy/h, about 1 DSB is produced every 2 h reducing the risk for repair errors due to the interaction of multiple DSBs. This scenario mimics radiation exposure of organisms that are living in the contaminated area where they are chronically exposed to LDR.
We have previously shown that low doses (in the mGy range) and low dose rates (in the range of 1 to 30 mGy/h) of gamma radiation are potent inducers of oxidative stress [31, 52]. It was also shown by other researchers that exposure of mice to repeated low-dose radiation may lead to radiation-adaptive response and tolerance to higher toxic doses. The suggested mechanism includes the induction of ROS. The response of the cells to certain levels of elevated ROS leads to the expression of antioxidant proteins and increased protection levels (adaptive response) as a consequence [53]. However, when ROS chronically elevated to high levels, the antioxidant levels may not be sufficient to neutralize the excessive levels of ROS, thereby resulting in redox homeostasis imbalance and modification of biomolecules including DNA and dNTP.
Previously, we showed that premature senescence could be induced by chronic LDR gamma radiation in primary human fibroblasts, as well as in primary human endothelial (HUVEC) cells [9, 16, 32]. By applying RNA-seq and proteome analysis, we showed that several key pathways such as PI3K/Akt/mTOR, IGFBP5 signaling, elevated oxidative stress in parallel with activation of immune response, and cytoskeletal reorganization were involved in stress-induced premature senescence [9, 15, 16, 17].
In order to find out if young and middle-aged primary fibroblasts respond
differently to radiation exposure in terms of oxidative stress and proliferation
rates, we exposed them to the LDR for 9 weeks. The results are presented in Fig. 2B and indicate that chronic irradiation slows down the PD of the middle-aged
cells (P13) by 50% at week 9, from 11.70
During LDR exposure, ROS are produced and can react with dNTP in the cytoplasm, producing different mutagenic modified dNTP such as 8-oxo-dGTP. A protein called hMTH1 dephosphorylates 8-oxo-dGTP to 8-oxo-dGMP, and then to 8-oxo-dG, which can be released from the cells to the extracellular environment to avoid the induction of mutation during replication [56]. Additionally, hMTH1 is a multifunctional protein involved in cell cycle arrest and PS [22]. Next, we wanted to investigate the level of hMTH1 in the PS and RS cells. The results presented on P19-ST cells in Fig. 3B, and P19-ST/P19-IR in Fig. 3C indicate that the levels of hMTH1 are not significantly changed by cell age or LDR exposure, although a non-significant decrease of both HO1 and hMTH1 were observed in P19-C and P23 cells. One explanation is that we measured only expression levels of hMTH1 and HO1, not the activity levels, and perhaps LDR exposure change the activity of the proteins. Another explanation is that other antioxidants that are more effective in neutralizing ROS than HO1 have been expressed by the cells due to several weeks of LDR exposure. The more effective antioxidants significantly reduce the levels of ROS which can cause no change in the levels of HO1 and hMTH1 in the LDR-exposed cells.
Furthermore, exposure to chronic oxidative stress from LDR exposure can lead to
a more extensive telomere length shortening than that of corresponding
LDR-non-irradiated control cells, thus slowing down the growth. The results
presented in Fig. 4A indicate that telomere lengths in P23 cells are
significantly shorter than in young P8 cells. Furthermore, LDR-irradiated P13
cells (P19-ST and P19-IR) have significantly shorter telomere lengths than the
corresponding control (P19-C). Very short telomeres can be recognized by the
cells as DNA damage which can lead to activation of DNA damage response and cell
cycle arrest and thus lower PD. The data indicate that exposure to chronic
oxidative stress induces telomere shortening which may slow down or/and inhibit
proliferation [57]. A linear relationship was indicated between telomere
shortening and the percentage of the SA-
Given that acute gamma radiation of 1 Gy induces 30–40 DSBs and 1000
single-strand breaks (SSBs) in total, 12 mGy/h will lead to approximately 8–9
DSBs and 200–300 single-strand breaks per cell per day and after 6 weeks of
exposure, a total number of about 350 DSBs and 10,000 SSBs per cell have been
induced. Due to the random distribution of DNA damage by ionizing radiation, some
of the DNA damage will end up in the telomeres. As the repair of DNA damage
generally is slower in senescent cells due to lower expression levels of DNA
repair proteins [30] than in young cells (as shown in Fig. 5A,B), the
steady-state level of DNA damage may be higher in the telomeres of senescent
cells and lead to activation of DNA damage signaling and probably cell cycle
arrest [21]. The results presented in Fig. 5B show that only a small fraction of
One of the important questions that we intended to answer in the present project was if RS and PS have similar characteristics. Using the same experimental design as previously published [9, 15, 17, 32], we exposed the P13 cells to LDR ionizing radiation for 6 weeks. One of the characteristics of senescence is that the cells are permanently/irreversibly arrested in the cell cycle. To confirm the irreversibility, following exposure to LDR, the cells were divided into two cell culture flasks, one was kept for 2 weeks in an incubator without radiation, allowing the cells to recover from the radiation effect (P19-ST). The cells in the other flask were kept under the same conditions as the first flask but in the incubator with continuous irradiation (P19-IR). The experimental design is important because by comparing the LDR effects between the P19-IR and P19-ST cells, we could investigate if the results obtained (effects of LDR exposure) are irreversible.
The results presented in Fig. 4A showed that P19-C, P19-ST, P19-IR, and P23 cells have significantly shorter telomere lengths as compared with P8 cells, confirming that telomere shortening is a marker of cellular aging. Notably, the P19-ST and P19-IR have also shorter telomere lengths than the P19-C control, indicating that LDR exposure (P19-ST and P19-IR cells) can result in telomere shortening and cause PS through induction of ROS and oxidative stress as a consequence [32]. Increased levels of ROS by LDR will lead to oxidative base damages and single-strand breaks in DNA, part of which can be localized in the telomeres, resulting in telomere shortening [63].
Considering SA-
It was reported that prolonged overexpression of P53, RB, P16, or P21 is sufficient to induce senescence [68]. In the present investigation, the P21 expression was determined as a marker of senescence. The results presented in Fig. 4E showed that P21 expressions were elevated in P19-C, P19-ST, P19-IR, and P23 cells as compared with the levels of that in the P8 cells. The results indicate that P21 is upregulated in all senescent cells and LDR exposure has no effects on the expression of P21. One explanation is that the level of P21 is already two folds upregulated and leveled off in the P19-C cells and the addition of LDR exposure (in P19-ST and P19-IR) cannot result in an additional increase of the P21 expression. P21 can induce and maintain the senescence condition of a cell [69].
Further, we exposed the cells acutely to 1 Gy and established their DNA repair
kinetics using the
Once the telomeres are shortened beyond a critical level, the proteins that form the Shelterin complex are unable to associate with the telomeric sequence and can no longer perform their role in capping the end of the chromosome. Therefore, the length is a major limiting factor in the function of telomeres. Interestingly, a decreased expression of DNA repair genes in senescent cells was reported, which may explain the accumulation of DNA damage in RS cells [30] but less is known about the accumulation of DNA damage and DNA repair kinetics of LDR-induced PS. The data indicate that elevated ROS levels in the RS, in parallel with a decreased expression of DNA repair genes and a less effective antioxidant system, may lead to an increased accumulation of DNA damage in RS.
We also found that senescent cells have a significantly larger nucleus size than the young cells (Fig. 4D). Nuclear enlargement was observed in senescent—glioma cells, primary astrocytes, and human fibroblasts [73, 74, 75]—and is suggested to be mediated by MAP kinases [74]. Although nuclear enlargement and alteration in nuclear structure do not appear to be a universal phenotype for senescence, the data suggest that nuclear enlargement may be an additional characteristic of cellular senescence [76].
In conclusion, our results showed that 6 weeks of chronic oxidative stress from
exposure to LDR initiates P13 cells to enter PS. The PS was confirmed by
determining telomere length and comparing it with control non-irradiated cells.
We also showed that: (a) the baseline levels of
The data are available upon request.
Conceptualization: TS, APK, EB, TR, PRG, SH and MHR; methodology: TS, APK, EB, TR, PRG; resources: SH and MHR ;writing and Original Draft Preparation: TS, APK, EB, TR, PRG SH and MHR; Critical review and Editing: TS, APK, EB, TR, PRG, SH and MHR; Supervision: SH and PRG. All authors read and approved the final manuscript. All authors have participated sufficiently in the work and agreed to be accountable for all aspects of the work.
Not applicable.
We would like to thank The Swedish Radiation Safety Authority for the economic support, associate professor Siv Osterman Golkar for valuable discussion, and our student Leo Westerberg for technical help with analyzing telomere lengths.
This work was supported by The Swedish Radiation Safety Authority, SSM.
The authors declare no conflicts of interest.
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