Snail modulates JNK-mediated cell death in Drosophila

Abstract

Cell death plays a pivotal role in animal development and tissue homeostasis. Dysregulation of this process is associated with a wide variety of human diseases, including developmental and immunological disorders, neurodegenerative diseases and tumors. While the fundamental role of JNK pathway in cell death has been extensively studied, its down-stream regulators and the underlying mechanisms remain largely elusive. From a Drosophila genetic screen, we identified Snail (Sna), a Zinc-finger transcription factor, as a novel modulator of ectopic Egr-induced JNK-mediated cell death. In addition, sna is essential for the physiological function of JNK signaling in development. Our genetic epistasis data suggest that Sna acts downstream of JNK to promote cell death. Mechanistically, JNK signaling triggers dFoxO-dependent transcriptional activation of sna. Thus, our findings not only reveal a novel function and the underlying mechanism of Sna in modulating JNK-mediated cell death, but also provide a potential drug target and therapeutic strategies for JNK signaling-related diseases.

Introduction

The Sna superfamily of transcription factors has been implicated in a broad spectrum of important biological functions, including mesoderm formation, epithelial–mesenchymal transition (EMT), tumor recurrence, immune regulation, neural differentiation, left–right identity, cell fate, and survival decisions^1–4. Most of the Sna family members share a similar organization, with a evolutionarily conserved C-terminal domain that contains four–six C₂H₂-type Zinc-fingers for DNA binding, whereas the N terminus with a SNAG (Snail/Gfi) domain harbors the repressor activity¹. As the first member of the Sna family, sna was identified as a critical regulator of mesoderm development in Drosophila melanogaster^5–7. Although lacking the SNAG domain, Drosophila Sna has a consensus Pro-X-Asp-Leu-Ser-X-Lys (P-DLS-K) motif and executes its repressive function via interacting with a co-repressor, carboxy-terminal-binding protein (CtBP)^8,9. As such, the fruit fly offers opportunities to investigate the physiological functions of Sna during development.

The c-Jun N-terminal Kinase (JNK) signaling is evolutionarily conserved from fruit fly to human, and plays crucial roles in regulating a wide range of cellular activities including proliferation, differentiation and migration, especially cell death^10,11. This pathway can be triggered by various extrinsic and intrinsic signals, and is mediated through a mitogen-activated protein kinase (MAPK) cascade¹². In Drosophila, the tumor necrosis factor (TNF) ortholog Eiger (Egr) binds to its receptor Grindelwald (Grnd), which in turn activates the conserved JNK cascade including dTAK1 (JNKK kinase), Hemipterous (Hep, the JNK kinase) and Basket (Bsk, the Drosophila JNK)^13–17. Upon activation, Bsk phosphorylates and activates downstream transcription factors including the forkhead box O (FoxO), which modulates UV-induced Bsk-mediated cell death by directly up-regulating the pro-apoptotic gene hid expression^18,19. Although tremendous effort has been made to complete the regulatory network centered on Egr-Bsk pathway in cell death^20–24, the down-stream regulators and the underlying mechanisms remain poorly understood.

In this study, we used Drosophila melanogaster as an excellent in vivo system and identified Sna as a novel modulator of JNK pathway. First, our genetic analysis indicates that Sna functions downstream of JNK to regulate ectopically activated JNK-induced cell death in eye and wing development. We further show that loss of sna can block physiologically activated JNK signaling-induced cell death, and that Sna is necessary and sufficient for JNK-induced puc expression. Moreover, we demonstrate that Sna modulates dFoxO-triggered cell death. Finally, we provide evidence that gain of JNK signaling promotes dFoxO-dependent sna transcription. In conclusion, these findings reveal a previously unrecognized function of Sna in JNK signaling-mediated cell death, in addition to its well-accepted roles in development and EMT.

Results

Depletion of sna suppresses ectopic Egr-induced cell death in development

Ectopic expression of the TNF ortholog Egr in Drosophila eyes driven by GMR-GAL4 (GMR > Egr) produces a small eye phenotype in the adult stage (Fig. 1b, c)^14,15. and triggers apoptotic cell death posterior to the morphogenetic furrow (MF) in third instar eye discs, as revealed by acridine orange (AO) staining that detects dying cells (Fig. 2a, b)²⁵, and anti-CDcp-1 antibody staining that specifically recognizes the cleaved effector caspase Dcp-1 (Supplementary Fig. 1a, b)²⁶. As the fly eye is also the most accepted organ of the nervous system²⁷, to quantify the extent of Egr-induced neuronal loss, we employed the UAS-mCD8-RFP (a fusion protein between mouse lymphocyte marker CD8 and the fluorescence protein) reporter system²⁸, and found that ectopic Egr resulted in remarkable loss of the photoreceptor neurons in Drosophila adult eyes (Fig. 1j, k, m).

Fig. 1. A genetic screen for dominant modifiers of GMR > Egr-induced eye-ablation phenotype.

a A schematic depiction of the genomic region surrounding the sna locus. The three deficiencies Df(2L)ED1050, Df(2L)ED1054, and Df(2L)Exel7063 are indicated. b–i Light micrographs of Drosophila adult eyes are shown. Compared with GMR-GAL4 control b, the GMR > Egr small eye phenotype c is considerably suppressed by deficiency Df(2L)ED1050 d, Df(2L)ED1054 e, or Df(2L)Exel7063 f that deletes genes including sna, or in heterozygous sna mutant g, or by expressing two independent sna RNAi h and i. The sample size of Drosophila adult eye is 50. j–l Representative fluorescent microscopy images of adult eyes are shown. m Statistical analysis of fluorescence signals (n = 10) shown in figures j–l. Error bars indicates standard deviation. One-way ANOVA with Bonferroni multiple comparison test was used to compute P-values, ^***P < 0.001. See the electronic supplementary material for detailed genotypes. Scale bar: 100 μm in b–i, 50 μm in j–l.

Fig. 2. Depletion of sna suppresses Egr-triggered cell death in development.

a–e Fluorescence micrographs of third instar larval eye discs are shown. Compared with the controls a, GMR > Egr-induced cell death in eye discs b remains unaffected by expression of a GFP RNAi c, but is dramatically impeded by knocking down sna d and e. f Statistical analysis of cell death in eye discs (n = 10) shown in figures a–e. Light micrographs of Drosophila adult wings g–k and fluorescence micrographs of third instar larval wing discs m–q are shown. Compared with the controls g and m, ectopic expression of Egr driven by ptc-GAL4 generates a loss-of-ACV phenotype in adults h and cell death in larval wing discs n, which are strongly blocked by RNAi-mediated depletion of sna j, k, p and q, but not that of GFP i and o. The lower panels show high magnification view of the boxed areas in upper panels g–k. Statistical analysis of the ACV phenotype in figures g–k (l, n = 20 for each genotype) and cell death in wing discs in figures m–q (r, n = 10) are shown. Error bars indicates standard deviation. One-way ANOVA with Bonferroni multiple comparison test was used to compute P-values, ***P < 0.001; ns, no significant difference. In all wings, anterior is to the left and distal up. UAS-GFP-IR is included c, i, o as a negative control to demonstrate that the suppressive effect of UAS-sna-IR is specific, but not a result of GAL4 titration by another UAS line. See the electronic supplementary material for detailed genotypes. Scale bars: 50 μm in a–e, g–k (lower panels) and m–q, 100 μm in g–k (upper panels).

To identify additional factors that regulate Egr-induced cell death, we performed a genetic screen for dominant modifiers of the GMR > Egr-induced small eye phenotype using the Bloomington Drosophila Stock Center Deficiency kit^21–24,29. One of the suppressors was mapped cytologically within 35D2-35D4, a region uncovered by three overlapping deficiencies Df(2L)ED1050, Df(2L)ED1054, and Df(2L)Exel7063 (Fig. 1a). Amalgamating such deficiency into GMR > Egr background significantly suppressed the reduced eye size (Fig. 1d–f). This region contains nine genes including snail (sna) (Fig. 1a), the Drosophila ortholog of Sna superfamily¹, which encodes a C₂H₂ zinc finger transcription factor involved in embryonic mesoderm development, EMT and asymmetric cell division^5,30–34. Intriguingly, the GMR > Egr eye phenotype was suppressed to a similar extent in heterozygous sna mutants (Fig. 1g), suggesting loss of sna is responsible for the suppressive effect of the deficiencies. Consistently, GMR > Egr triggered small eye phenotype, cell death, and photoreceptor loss were notably inhibited by two independent sna RNA interference (RNAi) that target distinct regions of the sna transcript (Fig. 1h, i, l, m; 2d–f; Supplementary Fig. 1d–f). A quantitative reverse transcription polymerase chain reaction (qRT-PCR) assay was performed to verify the knockdown efficiencies of the two sna RNAi lines (Supplementary Fig. 2a). A GFP RNAi was employed as a negative control (Fig. 2c; Supplementary Fig. 1c). Collectively, these results indicate that the transcription factor Sna plays an essential role in ectopic Egr-triggered cell death during eye development.

In Drosophila, sna, esgcargot (esg) and worniu (wor) are considered to be functionally redundant Snail superfamily members that encode zinc finger transcription factors^1,35,36. Although esg and wor are located in the vicinity of sna on the chromosome, they are not included in the region uncovered by Df(2L)Exel7063 (Fig. 1a). We found that GMR > Egr-induced small eye phenotype was not visibly suppressed by depletion of esg or wor (Supplementary Fig. 2e–j), suggesting that esg and wor are not involved in Egr-induced cell death.

To examine whether Sna plays a more general role in cell death, we expressed the pro-apoptotic gene head involution defective (hid) by the GMR-GAL4 driver³⁷, and found that GMR > Hid-induced small eye phenotype was not suppressed by knockdown of sna (Supplementary Fig. 2b–d), suggesting Sna is specifically involved in Egr-triggered cell death.

Drosophila adult wing represents another excellent model system to investigate cell death in development. Consistent with previous reports, expression of Egr along the anterior/posterior (A/P) compartment boundary driven by patched (ptc)-GAL4 also resulted in apoptotic cell death, revealed by AO staining (Fig. 2c, n) and anti-Cleaved Caspase-3 (CC-3) antibody staining (Supplementary Fig. 1g, h), a read-out of the initiator caspase (Caspase-9-like) DRONC activity³⁸, and generated a loss of anterior cross vein (ACV) phenotype (Fig. 2g, h)^29,39, which was phenocopied by expressing the cell death gene grim²³. These phenotypes were considerably impeded by RNAi-mediated inactivation of sna (Fig. 2j–l, p–r; Supplementary Fig. 1j–l), but remained unaffected by expression of GFP-IR (Fig. 2i, o; Supplementary Fig. 1i), suggesting that Sna modulates ectopic Egr-promoted cell death in a non-tissue-specific manner.

Sna acts downstream of Bsk to modulate cell death

Egr triggers both JNK-dependent and JNK-independent cell death in development^14,15,21. To determine whether Sna is required for JNK-mediated cell death, we overexpressed dTAK1 (JNKKK) or Hep (JNKK) in the developing eyes. Eye-specific expression of dTAK1 driven by sevenless (sev)-GAL4 or a constitutive activated form of Hep (Hep^CA) driven by GMR-GAL4 promoted extensive cell death in third instar larval eye discs, which were visualized by terminal deoxynucleotidyl transferase dUTP nick-end labeling (TUNEL) staining that labels both apoptotic and necrotic cells (Supplementary Fig. 3a, f)^40,41, and generated rough eyes with reduced size (Fig. 3a, e)^29,42. These phenotypes were suppressed by knockdown of sna (Fig. 3d, h; Supplementary Fig. 3d, e, I, j), but not that of GFP (Fig. 3b, f; Supplementary Fig. 3b, g), while heterozygous bsk¹ mutants were included as a positive control (Fig. 3c, g; Supplementary Fig. 3c, h). In addition, expression of Puc, a phosphatase that negatively regulates Bsk activity⁴³, near fully suppressed the small eye phenotype produced by GMR > Hep^CA (Supplementary Fig. 4). Together, sna is indispensable for Egr-induced Bsk-mediated cell death in eye development.

Fig. 3. Sna acts down-stream of Hep in JNK-mediated cell death.

a–h Light micrographs showing Drosophila adult eyes. The small and rough eye phenotype resulted from ectopic expression of dTAK1 a or Hep^CA e is evidently suppressed by mutating one copy of endogenous bsk c and g, or knocking-down sna d and h, but not GFP b and f, which served as a negative control. i–p Light micrographs of Drosophila adult wings. Compared with the controls i and m, the wing phenotypes of Sd > Hep^WT j and ptc > Hep^WT n flies are suppressed by expressing a sna-IR l and p, but not GFP k and o. In m–p, the lower panels are high magnification of the boxed areas in upper panels. Statistical analysis of the adult wing size/wild type (WT) q (n = 10) and the ACV phenotype r (n = 20 for each genotype) as shown in figures i–l and m–p, respectively. One-way ANOVA with Bonferroni multiple comparison test was used to compute P-values, ***P < 0.001; ns, no significant difference. In all wings, anterior is to the left and distal up. See the electronic supplementary material for detailed genotypes. Scale bars: 100 μm in a–l and m–p (upper panels), 50 μm in m–p (lower panels).

To investigate whether Sna modulates Bsk-mediated cell death in other cellular contexts, we activated Bsk signaling in the wing or dorsal thorax. Ectopic expression of wild type Hep in the wing pouch driven by Scalloped (Sd)-GAL4 (Sd > Hep^WT) promotes broad-scale cell death²³ that results in severely reduced adult wing blade (Fig. 3i, j), which was significantly suppressed by depleting sna (Fig. 3l, q). Accordantly, ptc > Hep^WT-induced apoptosis in third larval wing discs (Supplementary Fig. 3k, l) and loss-of-ACV phenotype in adult wings (Fig. 3m, n) were inhibited by expressing a sna RNAi, but not GFP (Fig. 3o, p, r; Supplementary Fig. 3m–o). In addition, we found that expression of Hep driven by pnr-Gal4 (pnr > Hep^WT) triggers cell death in the thorax²² and produces a small scutellum phenotype, which is partially suppressed by depleting sna, but not GFP (Supplementary Fig. 5). Hence, we conclude that Sna regulates JNK-mediated cell death down-stream of Hep in a non-tissue-specific manner.

Moreover, ectopic expression of Bsk under the control of GMR-GAL4 generates a small and rough eye phenotype (Supplementary Fig. 6a, b), which is suppressed by knockdown of sna (Supplementary Fig. 6d), but not expression of GFP (Supplementary Fig. 6c), suggesting that Sna acts down-stream of the JNK cascade to modulate cell death. In addition, ectopic expression of Sna is sufficient to trigger a large scale of cell death in the eye and wing discs (Supplementary Fig. 6e–i, n, s–u), and produce a small eye phenotype in the adulthood (Supplementary Fig. 6j). Consistent with the notion that Sna acts downstream of Bsk, the GMR > Sna-induced cell death and eye phenotype could not be suppressed by expressing Bsk^DN, while sna-IR and LacZ served as positive and negative controls, respectively (Supplementary Fig. 6k–m, o–r).

sna is required for the physiological functions of Bsk

The above data imply that Sna acts as a crucial factor down-stream of Bsk to modulate cell death, yet it remains unknown whether Sna is involved in the physiological role of JNK signaling. To address this question, we knocked down puc, which encodes a JNK phosphatase that negatively regulates JNK activity⁴³, along the A/P compartment boundary of wing discs by ptc-GAL4 (ptc > puc-IR), and observed strong cell death accompanied with increased caspase activity in third-instar larval wing discs (Fig. 4f; Supplementary Fig. 7a), and loss-of-ACV in adult wings (Fig. 4a). All the phenotypes, resulted from the activation of endogenous JNK signaling, were blocked by knockdown of sna, while expression of a dominant negative Bsk (Bsk^DN) or LacZ served as a positive or negative control, respectively (Fig. 4bb–e, g–j; Supplementary Fig. 7b–d, i).

Fig. 4. sna is required for the physiological functions of Bsk.

Light micrographs of Drosophila adult wings a–d and fluorescence micrographs of third instar larval wing discs f–i and k–n are shown. RNAi-mediated down-regulation of puc along the A/P compartment boundary by ptc-GAL4 triggers the loss-of-ACV phenotype in adult wings a, which is resulted from cell death in larval wing discs f. Both phenotypes depend on endogenous Bsk c and h and Sna d and i. The bottom panels show high magnification views of the boxed areas in upper panels a–d. Knockdown of dlg along the A/P compartment boundary (ptc > dlg-IR) induces Bsk-dependent cell death k and m, which is significantly blocked by depletion of sna n. LacZ expression is used as a negative control b, g, and l. e, j, and o Statistical analysis of ACV phenotype (n = 20 for each genotype) and cell death in wing discs (n = 10) as shown in figures a–d, f–i, and k–n, respectively. Error bars indicates standard deviation. One-way ANOVA with Bonferroni multiple comparison test was used to compute P-values, ***P < 0.001; ns, no significant difference. In all wings, anterior is to the left and distal up. See the electronic supplementary material for detailed genotypes. Scale bars: 100 μm in a–d (upper panels), 50 μm in a–d (lower panels) and f–n.

It has been reported that loss of cell polarity promotes JNK-mediated cell death in development^44–46. In agreement with this view, knockdown of the cell polarity gene disc large (dlg) along the A/P compartment boundary by ptc-GAL4 (ptc > dlg-IR) induces severe cell death (Fig. 4k) and up-regulated caspase activity (Supplementary Fig. 7e) in third instar larval wing discs. Both phenotypes were appreciably blocked by depletion of sna or expression of Bsk^DN, but remained unaffected by the expression of LacZ (Fig. 4l–o; Supplementary Fig. 7f–i). Thus, these data indicate that Sna contributes to the physiological function of Bsk signaling in regulating stress-induced cell death in development.

Sna mediates FoxO-triggered cell death

The transcription factor forkhead box O (FoxO) is a known down-stream regulator of Bsk-mediated cell death in response to stress^18,19. Consistently, we found that GMR > Egr-induced cell death in eye discs and small eye phenotype were significantly impeded in heterozygous dFoxO^Δ94 mutants, or by RNAi-mediated knockdown of dFoxO (Fig. 5a–c, g–i, m), suggesting dFoxO also regulates Egr-triggered Bsk-mediated cell death. To investigate the mechanism by which Sna regulates JNK-mediated cell death, we examined the genetic interaction between sna and dFoxO. Over-expression of dFoxO driven by GMR-GAL4 triggers intensive cell death in third instar eye discs and produces adult eyes with reduced size (Fig. 5d, j)^18,44. We found that both phenotypes were dramatically suppressed in heterozygous sna mutants (Fig. 5e, k), and near fully blocked by RNAi-mediated depletion of sna (Fig. 5f, l). Moreover, we found dFoxO expression in wing development driven by ptc-GAL4, Serrate (Ser)-GAL4, or Scalloped (Sd)-GAL4 triggered extensive cell death and generated various wing defects in their corresponding areas, which are efficiently blocked by RNAi-mediated depletion of sna, but not that of GFP (Fig. 5n–w; Supplementary Fig. 8). Taking these data together, we conclude that Sna is required for FoxO-induced cell death in eye and wing development.

Fig. 5. Sna regulates FoxO-mediated cell death.

Light micrographs of Drosophila adult eyes a–f, adult wings n–q, and s–v and fluorescence micrographs of third instar larval eye discs g–l are shown. The small eye phenotype and massive cell death, produced by GMR > Egr a and g, are obviously suppressed in heterozygous dFoxO^Δ94 background b and h or by knockdown of dFoxO c and i. Expression of dFoxO driven by GMR-GAL4 results in reduced eye size and increased cell death in eye discs d and j, which are suppressed by mutating one copy of endogenous sna e and k or RNAi-mediated depletion of sna f and l. Compared with the controls n and s, the wing phenotypes of Ser > dFoxO o and Sd > dFoxO t flies are partially suppressed by depletion of sna q and v, but not that of GFP p and u. In all wings, anterior is to the left and distal up. Statistical analysis of AO staining m, the adult wing size/wild type (WT) r and w as shown in figures g–l, n–q, and s–v, respectively (n = 10). One-way ANOVA with Bonferroni multiple comparison test was used to compute P-values, ***P < 0.001; ns, no significant difference. See the electronic supplementary material for detailed genotypes. Scale bar: 100 μm in a–f, n–q and s–v, 50 μm in g–l.

Scutoid (Sco) was originally identified as a dominant mutation resulted from a chromosomal transposition that affects sna, and is regarded as a sna gain-of-function allele⁴⁵. Intriguingly, we found that GMR > dFoxO-induced small eye phenotype is notably enhanced in heterozygous Sco mutants (Supplementary Fig. 9), confirming that gain of Sna exacerbates FoxO-induced cell death.

JNK signaling activates sna transcription

The above data suggest that Sna is necessary and sufficient for Bsk-FoxO-signaling-induced cell death in development. Since FoxO encodes a transcription factor, we hypothesized that JNK signaling may activate sna transcription in a FoxO-dependent manner. To test this, we activated JNK signaling in the eye by ectopic expression of Egr or Hep, and checked sna mRNA level by the qRT-PCR assay. In support of our assumption, endogenous sna transcription was evidently up-regulated by ectopic Egr or Hep, and this activation was significantly blocked in heterozygous dFoxO^Δ94 mutants (Fig. 6a), suggesting that JNK-induced sna expression depends on dFoxO. Consistently, the level of sna mRNA was also dramatically up-regulated by ectopic expression of dFoxO, but remained unaffected by that of LacZ (Fig. 6a). Thus, we conclude that JNK signaling triggers FoxO-dependent transcriptional activation of sna, which is necessary and sufficient for JNK-mediated cell death in development.

Fig. 6. JNK signaling activates sna transcription.

Histogram showing the levels of sna a and c and wg b mRNAs as measured by qRT-PCR. Error bars represent standard deviation from three independent experiments. One-way ANOVA with Bonferroni multiple comparison test or unpaired two-tailed t-test was used to compute P-values, ***P < 0.001. Light micrographs of Drosophila adult eyes d–g. The small eye phenotype produced by GMR > Sna d is not suppressed by RNAi-mediated depletion of wg or dsh e–g. See the electronic supplementary material for detailed genotypes. Scale bar: 100 μm in d–g.

wingless (wg) is a recognized target of JNK pathway^24,46,47 and elicits expression of Sna family transcription factors in the peripheral fly eye⁴⁸. To further dissect the function of Wg in Egr/JNK/FoxO/Sna axis, we first performed the qRT-PCR assay to check wg mRNA level in GMR > Egr eyes. In line with the previous studies, we found that ectopic Egr is sufficient to activate wg transcription (Fig. 6b). Next, we checked whether Wg is required for JNK-mediated sna expression. To this end, we employed two independent wg RNAi and noticed a strong suppressive effects on the elevation of sna mRNA level triggered by Egr (Fig. 6c), but not that induced by FoxO (Fig. 6a), suggesting that Wg may contribute to Egr-induced sna transcription in parallel with FoxO. However, the GMR > Sna-induced small eye phenotype could not be blocked by knockdown of wg or disheveled (dsh) (Fig. 6d–g), which encodes a scaffold protein as the Wg transducer⁴⁹. Thus, we confirmed that wg is involved in Egr/JNK-mediated sna transcription, but not required for Sna-promoted cell death.

Sna induces puc activation in vivo

The above data suggest that Sna is a crucial downstream factor mediating JNK-dependent cell death. Next, to check if Sna could activate puc transcription in vivo, we examined the expression of puc-LacZ reporter by executing an X-Gal-staining assay⁴². Compared with the Sd-GAL4 control, expression of Hep^WT or Sna strongly induces up-regulation of puc-LacZ (Fig. 7a–c). Furthermore, the activation of puc in wing pouch along the A/P boundary triggered by ptc > Hep^WT could be moderately impeded by mutation in sna (Fig. 7d–f), suggesting Sna is both necessary and sufficient for JNK-mediated puc expression. Consistent with the genetic data that Sna acts downstream of Bsk, depletion-of-dlg-triggered JNK phosphorylation was inhibited by expression of Bsk^DN, but not that of a sna RNAi or LacZ (Fig. 7g–j).

Fig. 7. sna activates puc transcription in vivo.

a–f Light micrographs showing X-Gal staining of a puc-LacZ reporter in wing discs. Compared with the control a, overexpression of Hep^WT or Sna in the wing pouch notably upregulated puc transcription b and c. Compared with ptc-GAL4 d, the increased puc-LacZ expression triggered by Hep^WT along the A/P compartment boundary e is partially impeded in heterozygous sna mutant f. g–j Fluorescence micrographs of Drosophila third instar larval wing discs are shown. The elevated JNK phosphorylation induced by knockdown of dlg g and g′ remains unaffected by RNAi-mediated depletion of sna j and j′. LacZ and Bsk^DN expressions are used here as negative and positive controls, respectively h, h′, i and i′. See the electronic supplementary material for detailed genotypes. Scale bar: 50 μm in a–c, 20 µm in d–j.

Discussion

With the sophisticated genetic tools and conserved cell death machinery, Drosophila has been widely considered as an excellent model organism to unravel novel regulators of the cell death program during the last two decades^50–52. In this study, we took advantage of the fly genetics and identified Sna as a novel regulator of Egr-induced cell death from a deficiency screen. Our genetic epistasis analysis established Sna as a crucial downstream mediator of the Egr-JNK-FoxO signaling in cell death. Mechanistically, Egr-JNK pathway activates sna transcription via FoxO. Previous work has reported that Wg signaling elicits expression of Sna family transcription factors in eye peripheral retinal apoptosis⁴⁸. In addition, Zhang et al. reported that wg is required for GMR > Egr-induced cell death, and that wg expression is activated by Jun/Fos-mediated Egr-JNK signaling²⁴. Thus, we are curious if Wg is required for JNK-mediated sna transcription. Our data demonstrate that Wg also contributes to Egr-induced sna transcription, but is not involved in the FoxO-promoted sna expression. These data suggest that the Egr-JNK signaling activates sna transcription by at least two independent mechanisms: FoxO and Jun/Fos-Wg. Moreover, we found Sna is sufficient to activate puc transcription, implying JNK activates puc expression via multiple means. Intriguingly, different from the previously reported functional redundancy in development^1,36, the other two Drosophila Sna family proteins Esg and Wor are not involved in Egr-induced JNK-mediated cell death. Given the evolutionary conserved role of Sna and JNK, the data presented in this study may suggest a novel function of mammalian Sna family proteins in JNK-mediated cell death, in addition to its well-accepted roles in EMT, cell fate decision and survival.

Materials and methods

Fly strains

Flies were kept on a cornmeal and agar medium at 25 °C according to standard protocols. Drosophila strains used include: sna¹ (25127), sna¹⁸ (3299), UAS-sna-IR^B (28679), UAS-mGFP (32197), bsk¹ (3088), UAS-Bsk, UAS-dFoxO (9575), Ser-GAL4 (6791), Sco/CyO (2555), UAS-mCD8-RFP (32219), UAS-dsh-IR (31306), wor¹(3155), wor⁴ (25170) and the deficiency kit were obtained from Bloomington Drosophila stock center. UAS-sna-IR^V (6263), UAS-puc-IR (3018), UAS-dlg-IR (41136), and UAS-wg-IR^V (13352) were obtained from Vienna Drosophila RNAi center. UAS-wg-IR^N (4889R-4), UAS-esg-IR^N-1 (3758R-1), and UAS-esg-IR^N-2 (3758R-5) were received from Fly Stocks of National Institute of Genetics (NIG-FLY). UAS-GFP-IR (0355) and UAS-wor-IR (GL00186) were obtained from TsingHua Fly Center. GMR-GAL4⁵³; Sd-GAL4 and ptc-GAL4³⁹; UAS-Egr, UAS-Egr^W, and UAS-Hid¹⁴; UAS-Bsk^DN, UAS-Puc, and puc^E6942; sev-GAL4, UAS-dTAK1, UAS-Hep^CA, UAS-Hep^WT, UAS-LacZ, pnr-GAL4, and UAS-GFP^22,29,54; dFoxO^Δ94 and UAS-dFoxO-IR³⁹ were previously described. UAS-Sna^74b fly was a kind gift of J. Kumar. For all fly cross experiments, healthy unmated male and female parents were randomly assigned to different groups. Double-blinded method was employed during the experiments.

AO staining

Eye and wing discs were dissected from third instar larvae in PBST and incubated in 1 × 10⁻⁵ M AO for 5 min at room temperature prior to imaging as described²¹.

TUNEL staining

The wing and eye discs were dissected from wandering third-instar larvae in PBS. Discs were fixed in 4% paraformaldehyde for 30 min at room temperature and washed with PBS-Tx (0.3% Triton100) three times for 30 min. TUNEL staining was performed using the Fluorescein Cell Death Kit produced by Boster Company.

X-Gal staining

Wing discs were dissected from third instar larvae in PBST (1 × PBS pH 7.0, 0.1% Triton X-100) and stained for ß-galactosidase activity as described²¹.

qRT-PCR

TRIzol (Invitrogen) was used to isolate total RNA from 10 wing imaginal discs dissected from third instar larvae or 30 adult heads collected from freshly eclosed flies of indicated genotypes, and qRT-PCR was performed as previously described⁵⁵ using following primers:

For rp49 Sense: 5′-TACAGGCCCAAGATCGTGAA-3′

Antisense: 5′-TCTCCTTGCGCTTCTTGGA-3′

For sna Sense: 5′-ATGGCCGCCAACTACAAAAG-3′

Antisense: 5′-GCAAACTGTGAGTCCTTGGTC-3′

For wg Sense: 5′-CCAAGTCGAGGGCAAACAGAA-3′

Antisense: 5′-TGGATCGCTGGGTCCATGTA-3′.

Immunohistochemistry

Imaginal wing discs dissected from third instar larvae were collected in cold PBS and fixed in 4% paraformaldehyde. After proper washes, the wing discs were blocked in 10% horse serum, and stained with antibodies. The following antibodies were used: rabbit anti-Cleaved Dcp-1 (1:100, Cell Signaling Technology, Cat. #9578), rabbit anti-Cleaved Caspase-3 (1:200, Cell Signaling Technology, Cat. #9661), and rabbit anti-phospho-JNK (1:200, Calbiochem, Cat. #559309). Secondary antibody was goat anti-Rabbit-Cyanine3 (1:1000, Life technologies, Cat. #A10520). Vectashield mounting media (Vector Laboratories, Cat. #H-1500) was used for mounting.

Data and statistics

All data were verified in at least three independent experiments. Results are presented as bar graphs or scatter plots created using GraphPad Prism 6.0. A combination of unpaired two-tailed t-test and one-way ANOVA with Bonferroni’s multiple comparison test was used to calculate statistical significance. Center values’ as mean. Error bars indicates standard deviation. P value < 0.05 was considered significant. ns is not significant, P ≥ 0.05; * is P < 0.05; ** is P < 0.01; *** is P < 0.001. P values are included in the relevant figure legends.

Conflict of interest

The authors declare that they have no conflict of interest.

Supplementary information

Supplementary Information accompanies this paper at (10.1038/s41419-019-2135-7).