During radiologic or nuclear accidents, high-dose ionizing radiation (IR) can cause gastrointestinal syndrome (GIS), a deadly disorder that urgently needs effective therapy. Unfortunately, current treatments based on natural products and antioxidants have shown very limited effects in alleviating deadly GIS. Reserve intestinal stem cells (ISCs) and secretory progenitor cells are both reported to replenish damaged cells and contribute to crypt regeneration. However, the suppressed β-catenin/c-MYC axis within these slow-cycling cells leads to limited regenerative response to restore intestinal integrity during fatal accidental injury. Current study demonstrates that post-IR overexpression of TIGAR, a critical downstream target of c-MYC in mouse intestine, mounts a hyperplastic response in Bmi1-creERT+ reserve ISCs, and thus rescues mice from lethal IR exposure. Critically, by eliminating damaging reactive oxygen species (ROS) yet retaining the proliferative ROS signals, TIGAR-overexpression enhances the activity of activator protein 1, which is indispensable for initiating reserve-ISC division after lethal radiation. In addition, it is identified that TIGAR-induction exclusively gears the Lgr5− subpopulation of reserve ISCs to regenerate crypts, and intestinal TIGAR-overexpression displays equivalent intestinal reconstruction to reserve-ISC-restricted TIGAR-induction. Our findings imply that precise administrations toward Lgr5− reserve ISCs are promising strategies for unpredictable lethal injury, and TIGAR can be employed as a therapeutic target for unexpected radiation-induced GIS.
Unexpected radiation exposure during terrorist events (e.g., the use of “dirty bombs”), industrial or nuclear accidents (such as the nuclear disasters in Chernobyl and Fukushima) is a current and continuing threat to the future. Under homeostatic conditions, the rapid turnover of the intestinal epithelium is driven by leucine-rich repeat-containing G protein-coupled receptor 5 (Lgr5)high intestinal stem cells (ISCs), which are especially vulnerable to high-dose ionizing radiation (IR)1,2. A dose of 15 gray (Gy) of radiation is sufficient to abrogate the proliferative output of these mitotically active Lgr5high ISCs, and thus causes severe acute damage of the epithelial integrity2. Within 7 days of high-dose IR exposure, mice suffered from diarrhea, malabsorption and weight loss always die with complications known as gastrointestinal syndrome (GIS). Although prophylactic administrations have demonstrated some desirable effects on preventing stem cell exhaustion and epithelial disintegration induced by high-dose IR exposure3,4,5, the current post-IR treatments based on natural products and antioxidants have shown very limited effects on reversing stem cell death and the deadly GIS6,7,8.
Besides the high-proliferating and radiosensitive Lgr5high ISCs (i.e., crypt base columnar cells (CBCs)), a slow-cycling and injury-resistant pool of stem cells could be arisen to divide when the CBCs are depleted9,10. These rare “+4” position cells mainly include the reserve ISCs marked by lineage tracing analysis with polycomb complex protein 1 (Bmi1)-creERT11,12 and Lgr5+ label-retaining secretory progenitor cells which are regarded functionally distinct from reserve ISCs13,14. These radioresistant “+4” position cells are low-proliferative under homeostasis, while become proliferative from 3–4 days after high-dose radiation15,16. However, during lethal IR exposure, the CBCs are exhausted rapidly and the intestinal epithelium always disintegrates around 5 days after radiation, which happens even prior to effective “+4”-position-cell division and crypt regeneration. Hence, further elucidation of the mechanisms leading these quiescent cells to division after lethal IR-injury is required for mitigating fatal GIS.
The Wnt/β-catenin/c-MYC axis plays a central role in regulating the division of ISCs. However, the suppressed β-catenin/c-MYC pathway within “+4” position cells results in limited regenerative response within 3 days after lethal radiation16. Therefore, targeting β-catenin/c-MYC signal after lethal IR-injury may be potential countermeasures for accelerating the regeneration of these quiescent cells and the intestinal epithelium. TP53-induced glycolysis and apoptosis regulator (TIGAR), a downstream target of c-MYC in mouse intestinal crypts17, has been indicated to be a critical scavenger of reactive oxygen species (ROS), which promotes DNA damage repair and cellular redox balance during genotoxic stress18,19.
In the present study, we demonstrate that overexpression of TIGAR may be promising in ameliorating the intestinal architecture and survival during unpredictable lethal injury. Mechanistically, TIGAR acts as a turn-on switch that facilitates cell division of Lgr5− reserve ISCs in an activator protein 1 (AP-1) dependent manner, which remedies the β-catenin/c-MYC-inhibited “defect” of these cells and gears crypt regeneration efficiently after lethal IR-injury.
Restricted TIGAR-overexpression in reserve ISCs mitigates lethal GIS
TIGAR has been indicated to be crucial for efficient CBC proliferation under genotoxic stress20. However, the actively cycling CBCs are too radiosensitive to be rescued by post-IR treatment, always undergoing apoptosis within 12 h after lethal IR exposure20. Given that both of the reserve ISCs and Lgr5+ label-retaining secretory progenitor cells contribute to intestinal regeneration, mice containing the loxp-stop-loxp-Tigar cassette allele were crossed with Bmi1-creERT mice and Lgr5-EGFP-IRES-creERT2 (Lgr5-creERT2) mice, respectively (Fig. 1a; and Supplementary Fig. 1a). Immediately after 15-Gy whole abdominal irradiation (WAI) (Fig. 1b), restricted TIGAR-induction within Bmi1-creERT+ or Lgr5-creERT2+ cells was performed upon a single intraperitoneal injection of tamoxifen. Critically, Bmi1-creERT;H11-Tigar-2A-EGFP (Bmi1-creERT;H11-Tigar) mice revealed a significantly increased survival of 37.5% beyond 30 days post-WAI in comparison with the wild-type (WT) cohorts with 100% mortality within 7 days post-IR (Fig. 1c). Consistently, inducible TIGAR-overexpression dramatically attenuated the intestine shortening 5 days post-WAI (Fig. 1d, e). Histopathological analysis of the proximal small intestines (Fig. 1f) further confirmed that specific overexpression of TIGAR in reserve ISCs largely reversed crypt loss (Fig. 1g) and reduction of crypt size (Fig. 1h) after lethal irradiation. Lineage tracing analysis indicated a growing Bmi1-creERT+ lineage in regenerative crypts after lethal IR-injury (Fig. 1i, j). Using cultured mouse miniguts in vitro, i.e., epithelial organoids that preserved the in vivo cell-type distribution and kinetics of intestinal crypts and villi21,22, it was found that around 24.6 ± 3.05% of organoids derived from Bmi1-creERT;H11-Tigar mice were robustly labeled with GFP at 7 days after 12-Gy irradiation (a lethal dose for cultured intestinal organoids in vitro23) (Fig. 1k, l). The number of GFP-positive cells per organoid was 1.00 ± 1.80, 2.86 ± 4.61 and 4.16 ± 7.44 in Bmi1-creERT;H11-Tigar cohort by day 3, day 5 and day 7 post-IR, respectively (Fig. 1m), suggesting a continuous expansion of Bmi1-creERT+ population. By comparison, the restricted TIGAR-induction in Lgr5-creERT2+ cells in vivo revealed no discernible quantitative effects on reversing intestinal disintegration (Supplementary Fig. 1b–e) and WAI-induced lethality (Fig. 1n) when compared with their WT cohorts. In vitro lineage tracing analysis also demonstrated that the restricted TIGAR-induction within Lgr5-creERT2+ cells failed to promote intestinal organoid regeneration (Supplementary Fig. 1f, g), and Lgr5+ cells along with their progeny cells in Lgr5-creERT2;H11-Tigar-2A-EGFP (Lgr5-creERT2;H11-Tigar) organoids were abolished from 2 days onward after 12-Gy irradiation (Supplementary Fig. 1h). Altogether, our results disclosed that the restricted TIGAR-induction within Bmi1-creERT+ reserve ISCs but not Lgr5+ label-retaining secretory progenitors could gear intestinal regeneration and ameliorate mouse survival after lethal WAI.
TIGAR-induction exclusively gears Lgr5- reserve ISCs to regenerate crypts
By asymmetric division, a single reserve ISC could generate a daughter cell and an Lgr5+ CBC to replenish the active stem cell compartment15. The active CBCs then either generate transit-amplifying (TA) cells, which divide rapidly to produce large quantities of enterocytes, or differentiate into secretory progenitor cells which commit to Paneth cells, goblet cells, or enteroendocrine cells10. Principal component analysis of single ISCs reveals clear differences of reserve ISCs in comparison to Lgr5high CBCs24. However, nearly 20% of the Bmi1-creERT+ population is reported to exhibit an “Lgr5+” identity, a transition state between the quiescent reserve ISCs and the active CBCs10,24. In order to identify whether TIGAR-induced crypt regeneration originated in the Lgr5+ subpopulation of reserve ISCs or the Lgr5- ones, we sought to perform in vitro TIGAR-overexpression by adenovirus transfection. The transfection was performed by mechanical separating the organoids from Matrigel (Fig. 2a), and TIGAR was able to be efficiently overexpressed in 69.4 ± 5.08% of organoids at 1 day post transfection (Fig. 2b, c). During lineage cell tracing analysis, organoids derived from either Bmi1-creERT;Rosa26-mTmG mice (Fig. 2d) or Lgr5-creERT2;Rosa26-EYFP mice (Fig. 2e) were exposed to 12-Gy IR in vitro and then transfected immediately with an adenoviral vector expressing TIGAR. The 4-hydroxytamoxifen (4-OHT) stimulation was performed soon after replanting the organoids, and the progeny of total Bmi1-creERT+ reserve ISCs or offspring of Lgr5-creERT2+ subpopulations could be marked by fluorescence. As expected, TIGAR-overexpression facilitated the Bmi1-creERT+ cell-derived lineage following irradiation (Fig. 2f–h). Nonetheless, the Lgr5-creERT2+ subpopulation was not benefited by TIGAR-overexpression since the fluorescence was undetectable in the live organoids 3–5 days post IR (Fig. 2i–k). Consequently, it could be speculated that TIGAR-induction within Bmi1-creERT+ ISCs predominantly promoted the Lgr5- reserve ISCs, rather than the Lgr5+ subpopulations, to regenerate thus ameliorated intestinal integrity after lethal IR exposure.
TIGAR-induced crypt regeneration is AP-1 dependent
Our previous study has reported that TIGAR has a function of providing antioxidant defense and maintaining cellular redox balance, which potentially contributes to activating the nuclear transcriptional factors such as AP-119. In the present study, we undertook fluorescence-activated cell sorting (FACS) to enrich Bmi1-creERT+ reserve ISCs 1 day after 15-Gy WAI (Fig. 3a), so that the activity of AP-1 in the collected Bmi1-creERT+ cells could be examined. As shown in Fig. 3b, the c-Fos/AP-1 activity was significantly increased in TIGAR-overexpressing reserve ISCs, suggesting that AP-1 might be pivotal in TIGAR-induced intestinal hyperplastic response after lethal radiation. For further confirmation, a specific inhibitor of AP-1, 3-(5-(4-(cyclopen-tyloxy)-2-hydroxybenzoyl)-2-((3-hydroxybenzo[d]isoxazol-6-yl) methoxy) phenyl) propanoic acid (3-PA)25,26 was used in vivo (Supplementary Fig. 2a). It was found that 3-PA potently inhibited the AP-1 activity in TIGAR-overexpressing Bmi1-creERT+ reserve ISCs after 15-Gy WAI (Fig. 3c). Consistently, AP-1 abolishment dramatically abrogated TIGAR-induced intestinal regeneration (Fig. 3d–h) and attenuated mouse survival after lethal irradiation (Fig. 3i). Notably, the Bmi1-creERT+ lineage cells per TIGAR-overexpressing organoid as well as the percentage of GFP-positive organoids were significantly diminished by 3-PA treatment in vitro (Fig. 3j, k; and Supplementary Fig. 2b), suggesting that the AP-1 activity was indispensable for initiating TIGAR-geared division of reserve ISCs after deadly IR-injury.
TIGAR accelerates reserve ISCs toward division by limiting damaging ROS
It was noteworthy that redundant TIGAR activity failed to gear reserve-ISC division during homeostatic conditions. Upon a pulse of 4-OHT in vitro and TIGAR-overexpression within reserve ISCs, the morphology and dynamics of TIGAR-overexpressing organoids remained the same as that of WT cohorts (Supplementary Fig. 3a, b). The reason might be attributed to another “initiating signal”, which was essential for gearing reserve ISCs toward regeneration. It was reported that the proliferative ROS signal was pivotal for CBC division and proliferation27. With the administration of N-acetyl L-cysteine (NAC), a traditional antioxidant which indiscriminately scavenged the damaging ROS and pro-proliferating ROS, the regeneration of reserve ISCs was examined to determine whether IR-induced pro-proliferation ROS acted as “initiating signal” in accelerating reserve-ISC division. As shown in Fig. 4a–d, NAC treatment could only drive the Bmi1-creERT+ cell division to a limited extent, which was far away from that of TIGAR-overexpression did. In vitro analysis also revealed that the AP-1 activity within Bmi1-creERT+ cells after 12-Gy irradiation was modestly enhanced by the NAC administration, with the degree lagging far behind the TIGAR-overexpressing cohort’s (Fig. 4e, f). To confirm whether TIGAR-induced crypt regeneration was in a dose-dependent pattern, intestinal organoids derived from both homozygous Villin-creERT2;H11-Tigar+/+ (Villin-creERT2;H11-Tigar) mice (Fig. 4g) and heterozygous Villin-creERT2;H11-Tigar+/− mice (Fig. 4h) were irradiated and stimulated by 4-OHT immediately post-IR. Ki67-based immunofluorescence assay illustrated that both homozygous and heterozygous TIGAR-overexpressing miniguts moved to proliferative phases that were notable at 3–5 days after irradiation (Fig. 4i, j). The degree, however, in the homozygous TIGAR-overexpressing organoids was considerably higher than that in heterozygous ones (Fig. 4i, j), whose TIGAR expression level was between WT organoids and homozygous organoids. These data further confirmed that IR-induced pro-proliferating ROS, which was not scavenged by TIGAR, might be a critical “initiating signal” for gearing reserve ISCs toward regeneration. This mechanism also explained why preclinical treatments simply based on traditional antioxidants had very limited effects on reversing intestinal disintegration and lethal GIS.
Intestinal TIGAR-overexpression displays equivalent reconstruction to restricted TIGAR-induction
To determine whether TIGAR-overexpression within the entire intestinal epithelium could display a better regenerative response than restricted induction in reserve ISCs, Villin-creERT2;H11-Tigar mice were exposed to 15-Gy WAI. Based on this animal model, TIGAR could be induced simultaneously in both Bmi1-creERT+ ISCs and Lgr5+ secretory progenitor cells, and the potential synergistic effects on crypt regeneration of these TIGAR-overexpressing cells could be examined. Exactly, Villin-creERT2;H11-Tigar mice revealed a notable attenuation in intestinal length shortening (Fig. 5a, b) and a considerable amelioration in epithelial integrity (Fig. 5c) after 15-Gy WAI. Critically, the crypt regeneration (Fig. 5d, e) and survival rate (Fig. 5f) of Villin-creERT2;H11-Tigar mice resembled those of Bmi1-creERT;H11-Tigar mice after lethal irradiation, indicating that TIGAR-induction failed to promote Lgr5+ secretory progenitor cell division to support crypt regeneration, even if the reserve ISCs were already accelerated to proliferation. Furthermore, the data also revealed that the contribution of other epithelial populations to crypt regeneration might be vanishingly small. Actually, although crypt cells such as Alpi-CreER-marked TA cells are reported to repopulate the crypt compartment upon IR-injury, little evidence supports their functional importance in epithelial regeneration28. Meanwhile, IR-evoked apoptosis of intestinal crypts within 24 h post-WAI was almost the same no matter TIGAR was overexpressed or not (Fig. 5g–j), suggesting that the post-IR treatment applied in the current study failed to attenuate WAI-induced crypt cell death. Hence, it was summarized that the amelioration of intestinal integrity induced by TIGAR-overexpression after lethal IR-injury was predominantly attributed to the acceleration of Bmi1-creERT+ reserve-ISC division.
A two-stem cell model is supported by burgeoning studies from the small intestine, involving an actively cycling but radiosensitive stem cell and a long-lived, injury-resistant reserve pool of ISCs which is regarded to reside upstream of the high-proliferating CBCs11,24,29,30. Classic theories of radiobiology demonstrate that cell’s radiosensitivity is positively correlated with the proliferative activity. Indeed, relieving the proliferative suppression of the reserve pool of ISCs before irradiation can result in enhanced epithelial radiosensitivity and aggravated GIS16. Conversely, if the suppressed cell division of low-proliferating stem-like cells cannot be released in time, the intestinal integrity may also fail to be regenerated after lethal IR-injury. Using “cre-loxp” mouse model, the present study indicates the possibility of TIGAR-based post-IR treatment in accelerating reserve-ISC division and ameliorating mouse survival under grievous GIS.
To establish the involvement of TIGAR in driving the intestinal regeneration, we applied mouse models of which TIGAR could be efficiently induced 18 h after stimulation in vivo (Supplementary Fig. 4a–f). During WAI, the head, neck, thorax, and extremities were shielded to protect the bone marrow (Fig. 1b), thus inducing predominant GIS3,4. Single intraperitoneal injection of tamoxifen was performed immediately after 15-Gy WAI to induce TIGAR expression timely. After lethal WAI exposure, Bmi1-creERT;H11-Tigar and Villin-creERT2;H11-Tigar mice revealed equivalent amelioration of intestinal epithelial integrity (Fig. 5c–e) and mouse survival (Fig. 5f), indicating that TIGAR-overexpression primarily accelerated reserve ISCs toward division to reestablish the intestinal architecture after lethal irradiation. It is worth noting that biomarkers of “quiescent” reserve ISCs are also found in a subpopulation of Lgr5+ crypt cells, while around 20% of Lgr5+ intestinal cells are largely quiescent13,24. This quiescent Lgr5+ population is mainly comprised of the Lgr5+ (label-retaining) secretory progenitors and a subpopulation of the Bmi1-creERT+ reserve ISCs. Critically, by lineage cell tracing analysis, the feasibility of TIGAR-overexpressing quiescent Lgr5+ cells in rescuing mice from lethal GIS was ruled out (Fig. 2i–k; and Supplementary Fig. 1f–h). The mechanisms might be roughly attributed to the following two reasons. On the one hand, when compared with the exact quiescent Bmi1-creERT+ reserve ISCs, quiescent Lgr5+ cells were reported to demonstrate much fewer tracing events in response to injury13,14, which made effective crypt regeneration incapable after lethal WAI exposure. On the other hand, the Lgr5+ characteristics endowed these cells with higher radiosensitivity31, which made them already lose viability or undergo apoptosis before TIGAR was introduced (Fig. 5h, j). However, the present study does not eliminate the indispensability of the de novo-generated Lgr5high CBCs in intestinal regeneration after lethal IR-injury32.
Based on the lineage tracing analysis, a recent study indicated that the Bmi1+ cancer stem cells possessed an increased AP-1 activity that drove tumor recurrence33, suggesting that AP-1 played critical roles in endowing Bmi1-creERT+ stem cells with proliferative potential. In the present study, a classical inhibitor of AP-1, 3-PA, was used to demonstrate the mechanism of TIGAR-induced proliferation after lethal IR. A significant abrogation of Bmi1-creERT+ cell division, especially the first asymmetric division at the early stage (1 day) post-IR, was observed when the transcriptional activity of AP-1 was inhibited by 3-PA (Fig. 3j, k). Interestingly, AP-1 abolishment only dramatically abrogated the Bmi1-creERT+ lineage after irradiation, but did not affect the proliferative activity of CBCs during homeostatic conditions (Supplementary Fig. 2c, d). This finding suggests that the AP-1 activity is dispensable for CBC-like stem cells during homeostasis, which might attribute to the high proliferative activities of Lgr5high CBCs endowed by the Wnt/β-catenin signals31,34,35,36. This also suggested that TIGAR-induction remedied the β-catenin-inactivated “defect” of the low-proliferating reserve ISCs, which facilitated the acceleration of cell division and crypt regeneration after lethal IR-injury (Fig. 6). Mechanically, TIGAR-induced activation of c-Fos/AP-1 might be attributed to the increased phosphorylation of c-Fos, but not the upregulation of c-Fos expression.
In conclusion, the current study indicates that during unexpected disasters, quiescent Lgr5− reserve ISCs can be awakened timely by TIGAR/AP-1 activation to reestablish intestinal architecture and ameliorate mouse survival. Meanwhile, our work reveals an unexplored role of TIGAR in accelerating reserve ISCs toward regeneration, and the capability of TIGAR-induction in activating AP-1 demonstrates its significant advantage over traditional antioxidant treatments (Fig. 6).
Materials and methods
Mature male and female Villin-creERT2 mice (B6N.Cg-Tg(Vil1-cre/ERT2)23Syr/J), Bmi1-creERT mice (B6;129-Bmi1tm1(cre/ERT)Mrc/J), Lgr5-EGFP-IRES-creERT2 mice (B6.129P2-Lgr5tm1(cre/ERT2)Cle/J), Rosa26-EYFP mice (B6.129×1-Gt(ROSA)26Sortm1(EYFP)Cos/J) and Rosa26-mTmG mice (B6.129(Cg)-Gt(ROSA)26Sortm4(ACTB-tdTomato,-EGFP)Luo/J) were purchased from Jackson Laboratory (ME, USA). H11-Tigar mice (C57BL/6N-Igs2em1(CAG-LSL-Tigar-2A-EGFP)Cgen), (i.e., mutant mice carry a CAG-loxp-stop-loxp-Tigar-2A-EGFP-polyA insertion targeted to the mouse Igs2 (intergenic site 2; H11) locus) were generated by Cyagen Biosciences Company (Guangdong, China). All mouse lines were maintained and bred on mixed genetic background.
If not otherwise stated, only male mice were used and littermates were randomly and blindly allocated to experimental groups. All experiments were conducted at 8–10 weeks of age. Genotyping was performed following the protocols of Jackson Laboratory. The study was conducted in compliance with local animal welfare laws, guidelines, and policies. All procedures were approved by the ethic committee of Soochow University (Approval No. ECSU-2019000150).
Mouse irradiation and tamoxifen administration
Mice weighing between 24 and 27 g were anesthetized and treated with a single dose of 15-Gy WAI at a dose rate of 1.6 Gy/min using an X-RAD 320iX Biological Irradiator (Precision X-ray, North Branford, CT, USA). A 3-cm area of the mice containing the gastrointestinal tract was irradiated (irradiation field), shielding the head, neck and upper thorax as well as lower and upper extremities and protecting a significant portion of the bone marrow. Immediately after irradiation, mice were injected with tamoxifen intraperitoneally. Tamoxifen (Sigma, Cat#T5648) was dissolved in corn oil (Sigma, Cat#C8267) at a final concentration of 20 mg/ml. Cre enzyme was induced by single injection of tamoxifen at a dose of 4.5 mg per 20 g body weight. The schedules for tamoxifen administration and radiation as well as mouse grouping were provided in the relevant figure legends. If not otherwise stated, H11-Tigar mice were used as controls and were given similar doses of tamoxifen.
Survival rate and small-intestine length
After 15-Gy WAI, the survival rate of the mice was monitored every day for up to 30 days. For intestinal length measurement, mice died before day 5 post-WAI were excluded, and the mice alive were administered with euthanasia on day 5 after 15-Gy WAI to analyze the small intestinal length.
Histology of small intestine
At day 1, 3, 5 after 15-Gy WAI, mice were administered with euthanasia, and the proximal small intestines were excised for histology. Small intestine tissues were fixed in 10% neutral-buffered formalin overnight. After embedded in paraffin, tissues were cut into 5-μm sections for haematoxylin and eosin (H&E) staining and observation.
Western blot assay
Protein lysates were prepared in RIPA buffer (Thermo Fisher Scientific, Cat#89900), resolved via SDS-PAGE, and transferred onto polyvinylidene fluoride membranes (Millipore, Cat#ISEQ00010). The following primary antibodies were used: TIGAR (Abcam, Cat#ab62533), Caspase-3 (CST, Cat#9662), β-actin (Abcam, Cat#ab8226). After incubation with HRP-conjugated secondary antibodies, bands were detected and visualized by FluorChem M (ProteinSimple, San Jose, CA, USA).
Mouse small intestine was cut open longitudinally and washed with cold PBS. The villi were collected by scraping the intestine with a microscope slide and stored for protein analysis. While the remaining small intestine was cut into 5-mm pieces and incubated in PBS with 2 mM EDTA for 30 min at 4 °C. After incubation, the tissue fragments were separated by vigorous shaking. The supernatant enriched for crypts was passed through a 70-μm cell strainer (BD Falcon, Cat#352350). After centrifugation, the final fraction of intestinal crypts was used for further culture.
Isolated crypts were suspended with Matrigel (Corning, Cat#356231, growth factor reduced), which was overlaid by the organoid medium. Advanced DMEM/F12 (Thermo Fisher Scientific, Cat#12634-010) medium was supplemented with EGF 40 ng/ml (Peprotech, Cat#315-09-100), Noggin 100 ng/ml (Peprotech, Cat#250-38-5), R-spondin 500 ng/ml (Peprotech, Cat#315-32-5), N2 1× (Thermo Fisher Scientific, Cat#17502048), B27 1× (Thermo Fisher Scientific, Cat#17504044), and Y-27632 dihydrochloride monohydrate 10 μM (Sigma, Cat#Y0503). Intestinal crypts were cultured in the above mentioned media in Matrigel until further assay. For TIGAR-induction, 4-OHT (Sigma, Cat#T176) with a concentration of 10 nM was administrated in vitro. After 24 h, the medium was replaced by normal organoid culture medium, with organoids still in Matrigel.
Organoid irradiation and transfection
After 12-Gy irradiation in vitro, transfection of Tigar-overexpressing adenovirus (Adv-CMV-Tigar-3flag) was performed by mechanical separating the organoids from Matrigel, and 4-OHT (10 nM) was added into the medium soon after replanting the organoids. After 24 h, the medium was replaced by normal organoid culture medium.
After culturing, the intestinal organoids were planted on 35-mm glass bottom dishes (Thermo Fisher Scientific, Cat#150682) and fixed by 4% cold paraformaldehyde, washed with cold PBS and blocked in Blocking buffer (1× PBS, 5% anti-goat serum, 0.01% Triton X-100) for 1 h. Then the fixed organoids were successively incubated with anti-DDDDK tag primary antibodies (Abcam, Cat#ab1162) or anti-Ki67 primary antibodies (Abcam, Cat#ab15580) at 4 °C overnight and secondary antibodies (Abcam, Cat#ab150073) or (Abcam, Cat#ab150062) at room temperature for 90 min. For frozen-section staining, optimal cutting temperature compound (Leica, Cat#14020108926) embedded intestinal cryosections of 10–14 μm thickness were stained with the DAPI for 5 min at room temperature. The confocal images were acquired using an Olympus FV1200 confocal microscope (Japan).
Fluorescence-activated cell sorting (FACS)
The intestine was cut open longitudinally and incubated with 2 mM EDTA solution at 4 °C for 30 min to isolate intestinal crypts. To generate a single cell suspension, cells were incubated with Accutase (BD Biosciences, Cat#561527) at 37 °C for 10 min. Flow cytometry analysis was performed with CELL SORTER SH800S (SONY, Japan). Cells were gated for single cell based on the profiles of Forward-scatter area versus backward-scatter area (FSC-A vs. BSC-A) and forward-scatter height versus forward-scatter width (FSC-H vs. FSC-W). The size of the nozzle for all sorting is 100 µm.
Analysis of AP-1 activation
The DNA-binding activity of AP-1 was measured using the TransAM kits (Active Motif, Cat#44096). Nuclear extracts of Bmi1-creERT+ cells containing c-Fos/AP-1 factors were added into the multi-well plates precoated with consensus double-stranded DNA oligomers. After incubation, the transcription factor bound to DNA sequences was detected by using antibodies against c-Fos according to the manufacturer’s protocol. The absorbance was examined by a Microplate Reader (BioTek, Synergy2, Winooski, VT, USA).
3-PA and NAC treatments
3-PA (MedChem Express, Cat#HY-12270) was dissolved in polyvinylpyrrolidone. For in vivo administration, mice were administrated with 3-PA (120 mg/kg body weight, i.g.) daily for 4 consecutive days before 15-Gy WAI and the subsequent tamoxifen induction. For in vitro administration, 3-PA (10 μM) was added into the organoid growth medium 1 day before 12-Gy irradiation. For NAC treatment, the organoids were treated with NAC (Sigma, Cat#A8199) soon after the irradiation at concentrations of 1.5 mM or 4.0 mM, respectively.
Data were expressed as mean ± SD from three independent determinations. Differences between groups with similar variance were analyzed by Student’s t test. Kaplan–Meier survival analysis and log-rank comparison were performed for survival studies. Asterisks represent the p values as follows: *p < 0.05, **p < 0.01 and ***p < 0.001.
Mettler, F. A. & Voelz, G. L. Major radiation exposure–what to expect and how to respond. N. Engl. J. Med.346, 1554–1561 (2002).
Potten, C. S. Radiation, the Ideal cytotoxic agent for studying the cell biology of tissues such as the small intestine. Radiat. Res.161, 123–136 (2004).
Hu, B. et al. The DNA-sensing AIM2 inflammasome controls radiation-induced cell death and tissue injury. Science354, 765–768 (2016).
Saha, S. et al. Macrophage-derived extracellular vesicle-packaged WNTs rescue intestinal stem cells and enhance survival after radiation injury. Nat. Commun.7, 13096 (2016).
Cui, M. et al. Faecal microbiota transplantation protects against radiation-induced toxicity. EMBO Mol. Med.9, 448–461 (2017).
Stickney, D. R. et al. Preliminary clinical findings on NEUMUNE as a potential treatment for acute radiation syndrome. J. Radiol. Prot.30, 687–698 (2010).
Ghosh, S. P. et al. Amelioration of radiation-induced hematopoietic and gastrointestinal damage by Ex-RAD(R) in mice. J. Radiat. Res.53, 526–536 (2012).
Krivokrysenko, V. I. et al. Identification of granulocyte colony-stimulating factor and interleukin-6 as candidate biomarkers of CBLB502 efficacy as a medical radiation countermeasure. J. Pharmacol. Exp. Ther.343, 497–508 (2012).
Clevers, H. The intestinal crypt, a prototype stem cell compartment. Cell154, 274–284 (2013).
Yousefi, M., Li, L. & Lengner, C. J. Hierarchy and plasticity in the intestinal stem cell compartment. Trends Cell Biol.27, 753–764 (2017).
Sangiorgi, E. & Capecchi, M. R. Bmi1 is expressed in vivo in intestinal stem cells. Nat. Genet.40, 915–920 (2008).
Tian, H. et al. A reserve stem cell population in small intestine renders Lgr5-positive cells dispensable. Nature478, 255–259 (2011).
Buczacki, S. J. et al. Intestinal label-retaining cells are secretory precursors expressing Lgr5. Nature495, 65–69 (2013).
Li, N., Nakauka-Ddamba, A., Tobias, J., Jensen, S. T. & Lengner, C. J. Mouse label-retaining cells are molecularly and functionally distinct from reserve intestinal stem cells. Gastroenterology151, 298–310 e7 (2016).
Yan, K. S. et al. The intestinal stem cell markers Bmi1 and Lgr5 identify two functionally distinct populations. Proc. Natl Acad. Sci. USA.109, 466–471 (2012).
Chaves-Perez, A., Yilmaz, M., Perna, C., de la Rosa, S. & Djouder, N. URI is required to maintain intestinal architecture during ionizing radiation. Science364, 849 (2019).
Lee, P., Hock, A. K., Vousden, K. H. & Cheung, E. C. p53- and p73-independent activation of TIGAR expression in vivo. Cell Death Dis.6, e1842 (2015).
Bensaad, K. et al. TIGAR, a p53-inducible regulator of glycolysis and apoptosis. Cell126, 107–120 (2006).
Zhang, H. et al. Radiosensitization of glioma cells by TP53-induced glycolysis and apoptosis regulator knockdown is dependent on thioredoxin-1 nuclear translocation. Free Radic. Biol. Med.69, 239–248 (2014).
Cheung, E. C. et al. TIGAR is required for efficient intestinal regeneration and tumorigenesis. Dev. Cell25, 463–477 (2013).
Schuijers, J. et al. Ascl2 acts as an R-spondin/Wnt-responsive switch to control stemness in intestinal crypts. Cell Stem Cell16, 158–170 (2015).
Basak, O. et al. Induced quiescence of Lgr5+ stem cells in intestinal organoids enables differentiation of hormone-producing enteroendocrine cells. Cell Stem Cell20, 177–190 e4 (2017).
Ren, J. et al. A novel morphometry system automatically assessing the growth and regeneration of intestinal organoids. Biochem. Biophys. Res. Commun.506, 1052–1058 (2018).
Li, N. et al. Single-cell analysis of proxy reporter allele-marked epithelial cells establishes intestinal stem cell hierarchy. Stem Cell Rep.3, 876–891 (2014).
Ye, N., Ding, Y., Wild, C., Shen, Q. & Zhou, J. Small molecule inhibitors targeting activator protein 1 (AP-1). J. Med. Chem.57, 6930–6948 (2014).
Kamide, D. et al. Selective activator protein-1 inhibitor T-5224 prevents lymph node metastasis in an oral cancer model. Cancer Sci.107, 666–673 (2016).
Cheung, E. C. et al. Opposing effects of TIGAR- and RAC1-derived ROS on Wnt-driven proliferation in the mouse intestine. Genes Dev.30, 52–63 (2016).
Tetteh, P. W. et al. Replacement of Lost Lgr5-Positive Stem Cells through Plasticity of Their Enterocyte-Lineage Daughters. Cell Stem Cell18, 203–213 (2016).
Montgomery, R. K. et al. Mouse telomerase reverse transcriptase (mTert) expression marks slowly cycling intestinal stem cells. Proc. Natl Acad. Sci. USA108, 179–184 (2011).
Asfaha, S. et al. Krt19(+)/Lgr5(-) cells are radioresistant cancer-initiating stem cells in the colon and intestine. Cell Stem Cell16, 627–638 (2015).
Tao, S. et al. Wnt activity and basal niche position sensitize intestinal stem and progenitor cells to DNA damage. EMBO J.34, 624–640 (2015).
Metcalfe, C., Kljavin, N. M., Ybarra, R. & de Sauvage, F. J. Lgr5+ stem cells are indispensable for radiation-induced intestinal regeneration. Cell Stem Cell14, 149–159 (2014).
Chen, D. et al. Targeting BMI1(+) cancer stem cells overcomes chemoresistance and inhibits metastases in squamous cell carcinoma. Cell Stem Cell20, 621–634 e6 (2017).
Fevr, T., Robine, S., Louvard, D. & Huelsken, J. Wnt/beta-catenin is essential for intestinal homeostasis and maintenance of intestinal stem cells. Mol. Cell. Biol.27, 7551–7559 (2017).
de Lau, W. et al. Lgr5 homologues associate with Wnt receptors and mediate R-spondin signalling. Nature476, 293–297 (2011).
Sato, T. et al. Paneth cells constitute the niche for Lgr5 stem cells in intestinal crypts. Nature469, 415–418 (2011).
This study was mainly supported by the National Key R&D Program of China (No. 2017YFC0108604), the National Natural Science Foundation of China (Nos. 81602793, 31570850, 31770910, 81771949, 11775052, and 31770912), the Natural Science Foundation of Jiangsu Province (No. BK20150355), the Science and Technology Development Plan of Suzhou (No. sys2018015), the Opening Foundation of State Key Laboratory of Radiation Medicine and Protection (GZK1201805), and the Postgraduate Research & Practice Innovation Program of Jiangsu Province (KYCX18_2519).
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Chen, F., Zhang, Y., Hu, S. et al. TIGAR/AP-1 axis accelerates the division of Lgr5− reserve intestinal stem cells to reestablish intestinal architecture after lethal radiation. Cell Death Dis 11, 501 (2020). https://doi.org/10.1038/s41419-020-2715-6
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