1. Stem Cells and Regenerative Medicine
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CtBP impedes JNK- and Upd/STAT-driven cell fate misspecifications in regenerating Drosophila imaginal discs

  1. Melanie I Worley
  2. Larissa A Alexander
  3. Iswar K Hariharan  Is a corresponding author
  1. University of California, Berkeley, United States
Research Article
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Cite as: eLife 2018;7:e30391 doi: 10.7554/eLife.30391

Abstract

Regeneration following tissue damage often necessitates a mechanism for cellular re-programming, so that surviving cells can give rise to all cell types originally found in the damaged tissue. This process, if unchecked, can also generate cell types that are inappropriate for a given location. We conducted a screen for genes that negatively regulate the frequency of notum-to-wing transformations following genetic ablation and regeneration of the wing pouch, from which we identified mutations in the transcriptional co-repressor C-terminal Binding Protein (CtBP). When CtBP function is reduced, ablation of the pouch can activate the JNK/AP-1 and JAK/STAT pathways in the notum to destabilize cell fates. Ectopic expression of Wingless and Dilp8 precede the formation of the ectopic pouch, which is subsequently generated by recruitment of both anterior and posterior cells near the compartment boundary. Thus, CtBP stabilizes cell fates following damage by opposing the destabilizing effects of the JNK/AP-1 and JAK/STAT pathways.

https://doi.org/10.7554/eLife.30391.001

eLife digest

Some animals are more able to replace damaged tissue than others. A salamander, for example, can re-grow an amputated limb but a mouse or human cannot. After damage or injury certain types of cells are lost and need to be replaced by cells that are left behind. The remaining cells – or new cells that develop from them – must change their characteristics to better resemble the lost cells. This property, known as plasticity, needs to be controlled tightly. Excessive plasticity can result in forming tissues that are completely inappropriate for that location in the animal.

The fruit fly Drosophila melanogaster can be used to investigate plasticity during regeneration. Fruit fly larvae contain structures known as imaginal discs that can regenerate if damaged. Occasionally, when the imaginal discs regenerate, they produce the wrong kind of tissue.

Worley et al. set out to look for genes that would normally prevent such mistakes. Their search began with looking for flies with mutations that caused regeneration to go awry following damage. Specifically, Worley et al. looked for mutant flies that grew extra wings after a structure was damaged that would normally only generate a single wing. Once such flies had been found, further experiments were used to narrow down the search and confirm which gene was mutated.

This approach revealed that flies with mutations in the gene for a protein called CtBP (which is short for C-terminal binding protein) made more errors during regeneration and commonly regenerated inappropriate structures such as an extra wing. Importantly, mammals have very similar genes, but few researchers had previously studied if they also play a role in regeneration.

Worley et al. went on to show that CtBP dampens the activity of two signaling pathways (namely the JNK/AP-1 pathway and the JAK-STAT pathway), both of which promote plasticity. Thus, when CtBP levels are reduced, there is excessive plasticity.

These findings implicate CtBP as a regulator of plasticity during regeneration. This is an important first step in thinking of strategies that would allow researchers to guide and reshape the development of tissues during regeneration.

https://doi.org/10.7554/eLife.30391.002

Introduction

As development proceeds in multicellular organisms, cells become more restricted in developmental potential. This results initially from the expression of lineage-specific transcription factors and is then stabilized by heritable chromatin states that restrict accessibility of the transcriptional machinery to subsets of genes (Britten and Davidson, 1969; Levine, 2010; Allis and Jenuwein, 2016). The relative stability of these ‘epigenetic landscapes’ is thought to protect cells from patterns of gene expression that are inappropriate to that particular lineage. The paradigm that progressive restrictions in cell fate during development are unidirectional and irreversible was challenged by the demonstration that nuclei from differentiated cells could be reprogrammed to a more naïve state either by transferring them into an enucleated fertilized egg (Gurdon, 1962) or by expressing a combination of transcription factors (Takahashi and Yamanaka, 2006). Indeed, pluripotent stem cells have been derived from highly specialized cell types including neurons (Kim et al., 2011) and lymphocytes (Loh et al., 2009).

Even earlier, studies of Drosophila imaginal discs by Ernst Hadorn and colleagues showed that cells determined to one fate could switch to a very different fate. During embryogenesis, groups of cells at particular locations are specified to form particular imaginal discs (e.g. genital disc, wing disc, eye-antennal disc) depending on their location in the embryo (Cohen, 1993). Although these fates are determined during embryogenesis, disc cells do not differentiate to form adult structures until many days later, when metamorphosis occurs. To investigate the stability of the determined state, Hadorn’s group transplanted imaginal disc fragments into abdomens of female adult flies where regeneration occurred. Most often, the tissue generated was appropriate for the implanted imaginal disc. However, at low frequency, regeneration resulted in tissue that was appropriate for a different disc (e.g. leg disc tissue generated from a fragment of genital disc). Hadorn termed this phenomenon transdetermination (a switch from one determined state to another) (reviewed in [Hadorn, 1968; McClure and Schubiger, 2007; Worley et al., 2012]).

While transdetermination has been studied for years, many aspects are still mysterious. First, the fate change does not happen in a single cell, but rather, initiates in a small group of cells (Gehring, 1967; Hadorn et al., 1970; Maves and Schubiger, 1998). How a group of cells coordinately changes fate is not known. Second, certain fate changes seemed more likely than others. For example, genital-to-leg transformations or leg-to-wing transformations were far more frequent than transformations in the opposite direction. Third, transdetermination can be viewed as an aberrant form of regeneration that occurs following tissue damage and correlates with increased local proliferation (Sustar and Schubiger, 2005). Increased JNK activity, which is observed following damage (Bosch et al., 2005; Mattila et al., 2005; Bergantiños et al., 2010; Fan et al., 2014), reduces Polycomb-mediated repression and increases the frequency of transdetermination (Lee et al., 2005) as well as other types of fate changes (Herrera and Morata, 2014; Schuster and Smith-Bolton, 2015) by mechanisms that have not been elucidated. Finally, not all regions within a given disc have the same probability of undergoing a change of fate; Gerold Schubiger and colleagues described a region in the leg disc called the ‘weak point’ that has drastically higher rates of leg-to-wing transdetermination (Schubiger, 1971; Maves and Schubiger, 1995).

Our understanding of cell fate plasticity during regeneration is still at an early stage. Based on gene expression changes in regenerating discs, mutations in several candidate genes examined were shown to change the frequency of transdetermination, but the underlying mechanisms are not known (Klebes et al., 2005; McClure et al., 2008). To systematically screen for mutations that increase the frequency of cell fate changes during regeneration, we used a genetic system developed in our laboratory that reproducibly ablates a specific portion of the wing pouch and then allows it to regenerate (Smith-Bolton et al., 2009). We identified mutations in the gene encoding the transcriptional co-repressor, C-terminal Binding Protein (CtBP), and show that CtBP opposes the destabilization of cell fates during regeneration caused by JNK and the JAK/STAT pathway.

Results

To study changes in cell determination during regeneration, we used a genetic system to damage specific parts of imaginal discs and investigated genetic alterations that modify the response of surviving cells. Damage was induced by expressing the pro-apoptotic gene, eiger (UAS-egr) under the control of the wing pouch driver, rn-GAL4, with temporal control provided by a temperature-sensitive version of the transcriptional repressor GAL80, tub-GAL80ts (Figure 1A). At 18°C for 7 days, development occurs normally to an early point in the third larval instar. Then, a temperature shift to 30°C for 40 hr inactivates GAL80ts allowing UAS-egr expression, leading to a large amount of apoptosis in the wing pouch. A return to 18°C enables functional GAL80ts to stop the expression of UAS-egr and allows regeneration to proceed (Smith-Bolton et al., 2009). This system will hereafter be referred to as rnts>egr.

A system to study damage-induced cell-fate changes and a screen to identify genes that stabilize cell fates following damage.

(A) The rnts>eiger (rnts>egr) genetic system is used to induce temporally-controlled, tissue ablation in the wing pouch of larval wing imaginal discs. (B–C) Regeneration following ablation of the pouch typically results in viable adults with wings of relatively normal appearance. (D) Wing discs after 72 hr of recovery show regeneration of the pouch, shown here stained with antibodies to pouch marker Pdm2 and Wg. (E–F) In some genetic backgrounds, ectopic wings are observed following ablation. (E) An adult with ectopic wings on both sides. (F) The wing and the ectopic wing detached from one side. (G) Wing disc with an ectopic pouch after 72 hr of recovery. Ectopic wings and ectopic pouches are indicated with an asterisk (*). (H) Schematic of the screen of deletions encompassing most of the third chromosome for enhancers of ectopic wing formation. Each deletion was tested by crossing to rnts>egr. Density-controlled cultures were developmentally synchronized by collecting L1 larvae, shifted on day 7 from 18°C to 30°C for 40 hr. Adults were scored for ectopic wings. (I) Graph of frequency of adults with one or more ectopic wings for each deletion screened, arranged by relative location in the third chromosome (cytogenetic positions indicated). (J, K) Deletion screen data binned into classes for the entire screen (J) and subsets of different deletion collections (K).

https://doi.org/10.7554/eLife.30391.003

Following damage induced using rnts>egr, most wing discs regenerated the lost tissue and the adults eclosed with wing blades of relatively normal size and a thorax of normal appearance (Figure 1B,C). Wing imaginal discs after 72 hr of recovery from damage had regenerated wing pouches (Smith-Bolton et al., 2009) (Figure 1D). However, in several genetic backgrounds, additional wing tissue was observed arising from the thorax posterior to the normal wing, in the region of the scutellum, at frequencies approaching as high as 40% of adults (Figure 1E,F). Normal halteres were still observed, indicating that the ectopic wings were not generated by a haltere-to-wing transformation (such as those caused by mutations in the Hox gene Ubx). In these same genotypes, wing discs often had a second (ectopic) wing pouch protruding from the posterior side of the notum (Figure 1G).

A screen for mutations that increase cell fate plasticity following tissue damage identifies CtBP

The increased frequency of ectopic wings in some genetic backgrounds suggests that there are genes whose normal function includes the stabilization of cell fates during damage and regeneration. To identify such genes, we systematically screened 226 stocks bearing deletions of the third chromosome for their ability, when heterozygous, to increase the frequency of ectopic wings following egr-mediated damage and regeneration (Figure 1H). The frequency of adults with ectopic wings (EW) was scored for each deletion and graphed based on relative position of the deletion in the genome (Figure 1I). Taken together, these deletions covered approximately 90% of the euchromatic portion of chromosome 3. Of these 226 deletions tested, two were lethal, 91 elicited no EWs, 93 elicited the formation of EWs at a low penetrance (<10%), 28 showed an intermediate penetrance (>10%,<25%) and 12 showed a high frequency of EWs (>25%)(Figure 1J). Deletions from different deletion collections, Bloomington Stock Center (BSC), DrosDel Project (ED) and Exelixis (Exel) each had a similar breakdown of classes (Figure 1K). The score for each deletion tested is in (Supplementary file 1).

We focused on the 87D region, since multiple overlapping deletions allowed us to narrow the region of interest to a small number of genes. We then tested the available alleles and identified the responsible gene as C-terminal Binding Protein (CtBP). A small deletion (Df(3R)Exel8157) that spans CtBP caused EWs in 47% of adults (Figure 2A). A hypomorphic CtBP allele, CtBP03463, and a loss-of-function allele, CtBP87De-10 (which we will henceforth refer to by its protein truncating mutation CtBPQ229*) caused EWs in 22% and 42% of adults, respectively (Figure 2A). Mock ablation, with only either 1) rn-GAL4, tub-GAL80ts or 2) tub-GAL80ts, UAS-egr did not yield EWs (Figure 2A). EWs were attached to the scutellum and were often unable to flatten and appeared round (Figure 2B). The highest frequency of EWs occurred when the genetic damage was initiated on day seven after egg lay (AEL) in CtBPQ229*/+ mutants, while no EWs were observed in wild type on all days tested (Figure 2—figure supplement 1).

Figure 2 with 1 supplement see all
Loss-of-function mutations in C-terminal Binding Protein (CtBP) enhance the frequency of damage-induced ectopic wing formation.

(A) Frequency of ectopic wings (EW) following rnts>egr damage or mock ablation. EW scored in heterozygous genetic backgrounds for a wild-type Oregon R strain (wtOR), a deletion that spans CtBP (DEL = Df(3R)Exel8157), and two previously characterized alleles of CtBP, CtBP03463 and CtBPQ229*. Mock ablation controls 1) rn-GAL4, tub-GAL80ts (rnts>) and 2) tub-GAL80ts, UAS-egr (ts>egr), conducted in CtBPQ229*/+ genetic background. (B) An ectopic wing in CtBPQ229*/+ following ablation and regeneration. EW = ectopic wing, Sc = scutellum, W = wing. (C) A schematic of the two major protein isoforms of CtBP (short and long). The amino acid residues that correspond to codons at the CRISPR guide RNA target sites are indicated (148 and 334). (D) Frequency of EW following rnts>egr damage in a wild type isogeneic background (wtiso) and CRISPR-generated CtBP alleles (CtBPN148PY (N–to–PY), CtBP148Δ2 (Δ2)) in that background. (E) CtBPQ229*/+ wing imaginal disc following 72 hr of recovery stained with an antibody to Nubbin (Nub), a wing pouch marker (Ng et al., 1995). The ectopic pouch is marked with an asterisk (*). All bar graphs show averages between multiple experiments, error bars show standard deviations, and the numbers listed above the bars are the total adults scored.

https://doi.org/10.7554/eLife.30391.004

CtBP was originally identified as a protein that interacted with the C-terminus of the adenovirus E1A protein (Boyd et al., 1993). It has subsequently been shown to function as a transcriptional co-repressor in mammals and in Drosophila (Nibu et al., 1998; Zhang and Levine, 1999). While mammals have two paralogs of CtBP, reviewed in (Chinnadurai, 2003), the Drosophila genome contains a single CtBP gene. CtBP itself does not bind DNA. Rather, it associates with multiple DNA-binding proteins that possess a PxDLS motif, or related motif, including Hairy (Poortinga et al., 1998), Krüppel (Nibu et al., 1998) and Brinker (Hasson et al., 2001). The Drosophila CtBP gene has multiple spliced isoforms that are predicted to generate seven different proteins, which are usually grouped as short (379–386 aa) or long (473–481 aa) (Figure 2C).

To confirm that the increased frequency of EWs was in fact due to the disruption of CtBP, we used CRISPR/Cas9 to generate CtBP alleles on an isogenized Oregon-R third chromosome that did not cause EWs following damage (0%, n = 1892 adults) (Figure 2D). We generated two CRISPR guide RNAs that target regions spanning codons shared between all predicted protein isoforms, located at codon 148 and 334 (Figure 2C). The alleles recovered include a likely hypomorph, CtBPN148PY (three base pair insertion), which induced EWs in approximately 11% of adults and a suspected null, CtBP148Δ2 (frame shift inducing two base pair deletion), which induced EWs in approximately 20% of adults (Figure 2D). When compared to the isogenic parent chromosome, CtBP-/+ increases the frequency of EWs. Ectopic pouches were observed in CtBP-/+ wing discs following damage and recovery (Figure 2E).

Early molecular events in the formation of the ectopic pouch

To investigate what was triggering the formation of EWs, we focused on the early stages of ectopic pouch formation. Wingless (Wg) plays a key role in specifying the wing pouch in early development and is also upregulated during regeneration (Smith-Bolton et al., 2009). We compared Wg expression and apoptosis following damage in wild type (Figure 3A–C) and CtBPQ229*/+ (Figure 3D–F) discs. At 0 hr of recovery, both wild type and CtBPQ229*/+ discs had apoptotic cells and cellular debris (which stain for DCP-1) and high Wg expression around the damaged wing pouch. In the wild type discs, the normal notum Wg stripe was maintained (Figure 3A’–C’). In contrast, in ~45% of CtBPQ229*/+ discs (n > 50), there was a spot of increased Wg expression along the posterior edge of the notum, along with a disruption of the notum Wg stripe (Figure 3D’). Over the next 24 hr to 48 hr of recovery and regeneration, ~40% of CtBPQ229*/+ wing discs showed a domain of Wg expression accompanying morphological changes associated with the outgrowth of a wing pouch from the posterior edge of the notum (Figure 3E,F). Note that apoptosis was also detected in this region after 24 hr and 48 hr of recovery (Figure 3E’, F’).

Figure 3 with 5 supplements see all
The formation of ectopic pouches is marked by the activation of Wg and JNK at a secondary location.

(A–F) Wg and apoptosis visualized in wing discs following rnts>egr ablation of the pouch at different time points during recovery and regeneration (0 hr, 24 hr, and 48 hr after the downshift) for wild type (A–C) and CtBPQ229*/+ (D–F). Apoptotic cells and their debris stain with an antibody to cleaved Drosophila caspase-1 (DCP-1). (A’–F’) Higher magnification images of the notum region. The site of secondary pouch formation is indicated with an asterisk (*). The arrow in (D’) points to a region where the normal stripe of Wg expression in the notum is disrupted. (G–H) Damage-dependent wg enhancer, BRV-B-GFP, following rnts>egr damage at 0 hr recovery in wild type (G) and CtBPQ229*/+ (H) Boxed regions are shown at higher magnification in (G’–H’). (I) Frequency of ectopic wings (EW) in adults following rnts>egr damage with two (control) or one copy of the damage-dependent wg enhancer (wg1/+), in wild type and CtBPQ229*/+. (J) Frequency of EW in adults following overexpression of UAS-egr or UAS-wg alone, or UAS-egr and UAS-wg together driven by rnts> in wild type and CtBPQ229*/+. (K) Expression of dilp8-GFP (dilp8MI00727) in an undamaged disc. (L–N) Expression of dilp8-GFP in damaged discs after 0 hr of recovery for wild type (L) and CtBPQ229*/+ (M) and after 72 hr of recovery for CtBPQ229*/+ (N). (O) Graph of frequency of discs with a spot of dilp8-GFP expression at different time points of recovery (0 hr, 24 hr, 48 hr, 72 hr), along with the frequency of ectopic wings per side (or heminotum) in adults.

https://doi.org/10.7554/eLife.30391.006

During regeneration, wg expression is upregulated through a damage-dependent wg enhancer, which is JNK-dependent (Schubiger et al., 2010; Harris et al., 2016). We found that this damage-dependent wg enhancer (BRV-B-GFP) drives reporter expression at the area of fate change in a subset of CtBPQ229*/+ discs, but not in wild type (Harris et al., 2016), following rnts>egr damage (Figure 3G,H). In addition, the removal of one copy of the damage-dependent wg enhancer, which is deleted in the wg1 allele (Schubiger et al., 2010), reduced the frequency of ectopic wings (Figure 3I). This is consistent with the ectopic pouch forming in a similar manner to the regenerating wing pouch (Harris et al., 2016).

It is known that ectopic wing pouches can be generated by the constitutive expression of UAS-wg along the anteroposterior compartment boundary in the absence of damage (Ng et al., 1996). We determined that ptcts>wg expression initiated during the second instar triggered ectopic wings, but expression initiated during the third instar did not for both wild type and CtBPQ229*/+ (Figure 3—figure supplement 1). This is in contrast to the fate change triggered by rnts>egr in the third instar and suggests that Wg alone is insufficient to reprogram cell fates as the disc matures. In agreement with this finding, the overexpression of rnts>wg alone, or co-expression of rnts>egr and >wg did not enhance the frequency of ectopic wings (Figure 3J). Together, this suggests that other signaling pathways are critical for triggering ectopic wings at this point in development.

Since the BRV-B wg enhancer is activated by the JNK pathway, we examined other indicators of increased JNK signaling: AP-1-RFP (Chatterjee and Bohmann, 2012) and Matrix Metalloprotease 1 (MMP1) protein (Page-McCaw et al., 2003) expression. At 0 hr of recovery, both AP-1-RFP and MMP1 were expressed robustly around the egr-ablated wing pouch, and in many CtBPQ229*/+ discs, at a second location in the notum (Figure 3—figure supplement 2). AP-1-RFP activity was observed in an ectopic pouch at 48 hr of recovery (Figure 3—figure supplement 2), suggesting that JNK activity at the secondary site may be important for triggering ectopic wing pouch formation in CtBP-/+ mutants.

Previous studies found that dilp8 was highly upregulated during leg-to-wing transdetermination (Klebes et al., 2005) and also in regenerating imaginal discs (Katsuyama et al., 2015; Skinner et al., 2015; Harris et al., 2016). dilp8 encodes a secreted protein that is generated in response to abnormalities in tissue growth, likely in response to increased AP-1 activity, and Dilp8 expression delays pupariation (Colombani et al., 2012; Garelli et al., 2012; Colombani et al., 2015; Garelli et al., 2015; Vallejo et al., 2015; Jaszczak et al., 2016). A Minos insertion in the dilp8 locus, dilp8MI00727, functions as a transcriptional reporter of dilp8 via the expression of GFP, which we will refer to as dilp8-GFP. Under normal undamaged conditions, there was very low expression of dilp8-GFP in the wing disc (Figure 3K). As expected, damage with rnts>egr resulted in high dilp8-GFP expression around the damaged and regenerating wing pouch (Figure 3L). In a subset of CtBPQ229*/+ discs there was a second spot of dilp8-GFP expression in the notum at 0 hr of recovery (Figure 3M), which largely overlapped with the area of increased Wg expression. After 72 hr of recovery, dilp8-GFP was still detectable in a morphologically distinct outgrowth, which by this stage expressed Wg in the characteristic pattern of a mature wing pouch (Figure 3N). At 0 hr of recovery, dilp8-GFP expression in the notum overlapped with MMP1 expression (Figure 3—figure supplement 2), which is consistent with JNK activity contributing to dilp8-GFP expression. dilp8-GFP in the notum was expressed in cells that still expressed the hinge and notum marker Teashirt (Tsh) and before the pouch marker Nubbin (Nub) was detected (Figure 3—figure supplement 3) suggesting that it may be an early marker of an impending fate change in notum cells.

To determine if early dilp8-GFP expression in the notum was predictive of ectopic pouch formation, we quantified its frequency at different recovery time points in wild type and CtBPQ229*/+ discs and the frequency of EWs per side in adults (Figure 3O). The frequency of secondary dilp8-GFP spots was relatively constant across time points in CtBPQ229*/+ discs and absent in wild-type discs. In addition, the frequency of EW per adult heminotum roughly matched the frequency of dilp8-GFP spots in discs. Therefore, in this system, the secondary spot of dilp8-GFP expression in the notum is likely an early predictor of future ectopic pouch and ectopic wing blade formation.

Do the events that trigger ectopic wings occur independently between the two wing imaginal discs within one larva? We recorded the number of CtBPQ229*/+ adults with ectopic wings absent (63%), on one side (23%) and on both sides (14%) (Figure 3—figure supplement 4). Slightly more adults had bilateral ectopic wings than predicted for completely independent events. This could be due to identical timing of the discs or long-range signals (circulating factors) that simultaneously promote, or are permissive for, fate changes in both discs.

In support of the idea of possible circulating factors promoting a permissive environment for ectopic pouch formation, we found that as animals homozygous for the loss-of-function allele, dilp8MI00727, do not regenerate well (as seen in [Skinner et al., 2015]) and also lacked ectopic wings (EW) (Figure 3—figure supplement 5). Conversely, we found that the addition of UAS-dilp8 enhanced the frequency of EWs, without triggering EWs on its own (Figure 3—figure supplement 5). Together this suggests that a developmental delay is important for EW formation.

The ectopic wing pouch arises from cells in the notum

To determine if the ectopic pouch arises from a single cell changing its fate or from multiple cells, we generated marked clones of three varieties by hsFLP-induced recombination during the damage period and observed the clones following the growth of the ectopic pouch. The marked clones were arranged radially in the ectopic pouch yet only occupied a small fraction of it (estimated to be 10%) (Figure 4A). Thus, the ectopic pouch was generated either from multiple cells simultaneously changing fate or by the progressive recruitment of additional cells.

Figure 4 with 1 supplement see all
Characterization of the origin of cells that contribute to the ectopic pouch.

(A) rnts>egr, CtBPQ229*/+ wing disc with randomly-generated clones (two independent FLP-out constructs, Act<stop<lacZnls and Ubi<stop< GFPnls) generated with a 10 min heat-shock (37°C) at the start of the temperature shift from 18o C to 30o C and dissected 72 hr after the downshift. In (A’), there are three uniquely labeled clones (only Ubi-GFP, only Act-lacZ, or both), as indicated by arrowheads of matching color, in the ectopic pouch. (B–C) Lineage tracing following rnts>egr induced damage in wild type (B) and CtBPQ229*/+ (C) genetic backgrounds with R76B02-lexA, lexAOp-FLP, Ubi<stop<GFPnls after 72 hr of recovery. (D–F) rnts>egr, CtBPQ229*/+ wing discs with the enhancer trap mirr-lacZ stained with anti-Wg. (D) Undamaged. (E–F) Damaged discs, after 0 hr (E) and 72 hr (F) of recovery. N indicates notum, H indicates hinge. The asterisk indicates area of increased Wg expression in (E) and the ectopic wing pouch in (F). (G) Frequency of ectopic wings (EW) following rnts>egr damage in wild type or CtBP334Δ4/+ together with different mirr alleles, mirr1486/+ and mirr1825/+. Error bars show standard deviations. (H–J) rnts>egr, CtBPQ229*/+wing discs at different time points of recovery with dilp8-GFP, anti-Cubitus Interruptus (Ci) for marking the anterior compartment and anti-Engrailed (En) for marking the posterior compartment. Note that dilp8-GFP expression initiates in the posterior compartment and then spreads to the anterior compartment. (K) rnts>egr, CtBPQ229*/+ wing discs containing randomly generated marked clones (similar to A) that were induced on day 5 (48 hr before the temperature shift). Note the large GFP-positive clone in the posterior compartment of the ectopic pouch that abuts a significant portion of the anterior/posterior compartment boundary. Dotted boxes indicate areas that are enlarged in subsequent panels. The time of recovery (i.e. after downshift) is indicated in the bottom right corner of the relevant panel.

https://doi.org/10.7554/eLife.30391.012

To determine if the cells that give rise to the ectopic pouch had originated in the notum, we lineage-marked cells using the lexA system. This allowed us to use the GAL4/UAS system to ablate the pouch and to permanently label cells that expressed the lexA lines with lexAOp-FLP, Ubi<stop<GFPnls. R76B02-lexA was expressed primarily in the notum in the absence of damage (Figure 4—figure supplement 1). Following regeneration, a large number of notum cells were GFP labeled in the control discs (Figure 4B) and a significant proportion of the cells in the ectopic pouch was GFP labeled in CtBP-/+ discs (Figure 4C). Therefore, the cells that gave rise to the ectopic pouch once expressed R76B02-lexA, which indicates that these cells were once notum tissue, but had undergone a fate change to generate the ectopic pouch. Labeling with two additional lexA lines also supported the conclusion that a fate change occurred from notum to ectopic pouch (Figure 4—figure supplement 1).

A key transcription factor in the development of the notum is Mirror (Mirr) (Diez del Corral et al., 1999). The boundary between the notum and the hinge is located at a prominent fold at the edge of the mirr-lacZ expression domain (Wang et al., 2016) (Figure 4D). We observed the ectopic Wg expression in the notum within the mirr-lacZ expression domain (Figure 4E), and evidence of a new notum/hinge boundary in the ectopic growth (Figure 4F). In addition, removing one copy of mirr increased the frequency of ectopic wings in both wild type and CtBP mutant backgrounds (Figure 4G), suggesting that reducing the expression of notum-specifying factors increases the probability of damage-induced fate change, especially when CtBP levels are also reduced.

The ectopic pouch is derived from both anterior and posterior cells

The ectopic pouch was usually composed of both anterior (A) and posterior (P) cells, yet the initial events appeared to occur near the posterior edge of the disc, raising the possibility that posterior cells might have changed to an anterior identity. Indeed, when we examined dilp8-GFP expression in discs following ablation, with the A and P compartments visualized, we found that the entire cluster of dilp8-GFP expressing cells was usually located posterior to the compartment boundary (Figure 4H). For discs at 0 hr of recovery with dilp8-GFP or AP-1-RFP expression in the notum, the expressing cells were scored as P in 17/20 discs, as A in 2/20 discs and as both A and P in 1/20 discs. Then, during the growth of the ectopic pouch, dilp8-GFP expression was observed in both A and P cells (Figure 4I,J). When we labeled individual cells two days prior to the ablation and examined the clones that they generated, we found that even large clones in the ectopic pouch did not cross the compartment boundary (n = 7) (Figure 4K). Therefore, the ectopic pouch was likely generated from both A and P precursor cells.

Taken together, these experiments show that the ectopic pouch arose from a group of cells in the notum that is composed of both A and P cells. These cells collectively underwent a notum-to-pouch fate change while preserving their compartmental identities. The appearance of the dilp8 expression first in the P compartment and later in the A compartment suggests that the initial fate change recruited cells from across the compartment boundary to generate the ectopic pouch.

Re-specifying cell fates requires the activation of the JNK/AP-1 pathway

We have shown that JNK signaling was increased in the notum at an early stage in the development of an ectopic pouch. Moreover, our system is based on the targeted expression of Egr, which is the Drosophila Tumor-Necrosis Factor-α (TNF-α) ligand that activates JNK-dependent apoptosis (Igaki et al., 2002) in the wing pouch. Thus JNK-signaling may function in multiple ways to promote the notum-to-pouch fate change. To test if JNK signaling was required, we reduced JNK signaling either throughout the disc or only within the GAL4-expressing domain. The removal of one copy of the gene encoding the JNK kinase, hemipterous (hep), reduced the frequency of ectopic wings (Figure 5A). Blocking JNK signaling autonomously in the rn-GAL4 domain with the expression of a dominant negative form of JNK (>JNKDN) or of the AP-1 transcription factor Fos (>FosDN) completely suppressed the formation of ectopic wings (Figure 5A), and also reduced the ablation of the wing pouch (Figure 5—figure supplement 1). Thus, JNK/AP-1 signaling was needed for the generation of ectopic wings, either through JNK-mediated apoptosis or other JNK-mediated signaling events.

Figure 5 with 7 supplements see all
Egr activation of the JNK pathway is required for the formation of ectopic wings.

(A) Frequency of ectopic wings (EW) following rnts>egr damage in wild type or CtBP334Δ4/+ (CtBP334Δ4 was generated via CRISPR/Cas9 on the same chromosome that contains rnts>egr) in listed genotypes: (1) hepr75/+, (2) co-expression of UAS-JNKDN and (3) co-expression of UAS-FosDN. (B) Frequency of ectopic wings (EW) following rnts> expression of listed transgenes (UAS-rpr, UAS-hepwt, UAS-hepCA, UAS-grindICD, UAS-ecto-egr) in wild type and CtBP-/+ genetic background. Temperature shifts for experiments shown in (A) and (B) were done on day 7 AEL for 40 hr. (C–H) Wing discs with homozygous mutant clones of FRT82B CtBPQ229* generated by mitotic recombination with the transcriptional reporters for AP-1-GFP (C, D), MMP1-lacZ (E, F) and dilp8-GFP (G, H).

https://doi.org/10.7554/eLife.30391.014

We found, however, that ablation of the pouch alone was not sufficient to produce ectopic wings, as the expression of the pro-apoptotic gene reaper (rpr) did not produce ectopic wings, even in a CtBPQ229*/+ background (Figure 5B). Although rnts>rpr leads to a more effective ablation of the wing pouch than rnts>egr, it does not activate JNK to the same levels (Smith-Bolton et al., 2009; Harris et al., 2016). We tested if cell-autonomous methods of increasing JNK activity would lead to ectopic wings by expressing either a wild-type or constitutively active form of hep (rnts>hepwt, rnts>hepCA) (Figure 5B). Ectopic wings were only observed at very low frequency with rnts>hepCA, which could conceivably be the result of cell non-autonomous JNK activation via Egr expression (Pérez-Garijo et al., 2013). Reducing the amount of apoptosis by shortening the ablation period from 40 hr to 24 hr reduced the frequency of EW for rnts>egr from ~45% to ~11% in CtBPQ229*/+, and did not produce any EWs for either rnts>rpr or rnts>hepCA (Figure 5—figure supplement 2). Egr signals through the receptor Grindelwald (Grind) to activate JNK signaling (Andersen et al., 2015). Overexpression of the intracellular domain of Grind (rnts>grindICD) induced apoptosis, yet did not produce EWs (Figure 5B). However, expression of a secreted form of Egr (rnts>ecto-egr) (Narasimamurthy et al., 2009), caused EWs at a slightly higher frequency than the full-length (membrane-tethered) form (Figure 5B). Thus, while the ablation of the pouch by Egr was necessary for the formation of EWs, some local spread of Egr also appeared necessary.

In order to determine where egr must be expressed to trigger ectopic pouch formation, we closely examined the expression domain of rn-GAL4 with G-TRACE and detected expression in the wing pouch, a subset of the myoblasts and, at low levels, in scattered notum cells (Figure 5—figure supplement 3). Experiments with other GAL4 drivers determined that the expression of egr in the pouch was critical to the formation of ectopic wings and that the expression of egr in the notum or myoblasts was not sufficient (Figure 5—figure supplement 3).

Egr signaling activates both JNK signaling and apoptosis. While it is difficult to separate high-JNK activity from apoptosis, reducing apoptosis either by removing one copy of the pro-apoptotic genes rpr, hid, and grim (deleted in Df(3L)XR38), or by co-expressing a dominant-negative form of an effector caspase (>DroncDN) did not affect EW frequency (Figure 5—figure supplement 4). Co-expression of the anti-apoptotic gene UAS-p35 with rnts>egr, still generated EWs in the adults (Figure 5—figure supplement 4). Conversely, increasing apoptosis by co-expression of rnts>ecto-egr and rnts>rpr suppressed the formation of ectopic wings. This suggests that a population of cells that experienced increased JNK signaling without dying quickly was needed. Such cells in the pouch could be a source of diffusible factors that promote cell fate re-specification in the notum. We observed evidence for cells that experience Egr expression and yet survive in both the regenerated wing pouch and the ectopic pouch; cells forming the ectopic pouch may activate rn-GAL4 as they adopt a wing pouch fate (Figure 5—figure supplement 5).

CtBP expression was uniform in undamaged and damaged wing discs (Figure 5—figure supplement 6). Rescue was achieved when additional CtBP was expressed throughout the disc, but not when only expressed in the wing pouch (Figure 5—figure supplement 6). In addition, the knockdown of CtBP in the rn-GAL4 domain during damage did not result in ectopic wings (Figure 5—figure supplement 6). Therefore CtBP likely functions outside the rn-GAL4 domain, possibly in the notum, to prevent damage-induced ectopic wings.

Does a reduction in CtBP gene dosage affect JNK signaling? CtBP mutant clones in wing imaginal discs autonomously upregulated AP-1 targets AP-1-GFP (Figure 5G), dilp8-GFP (Figure 5H), and MMP1-lacZ (Figure 5I) but did not cause detectable apoptosis or elevated levels of MMP1 protein (Figure 5—figure supplement 7). Interestingly, the activation of AP-1-GFP and dilp8-GFP was not uniform within the mutant clones or between clones, and clones in the hinge often showed higher levels of activation. Thus, reducing CtBP protein levels could enhance JNK signaling especially in some regions of the disc.

JAK/STAT signaling promotes the re-specification of cell fates

Since the experiments with manipulations of the JNK pathway pointed to diffusible factors that were produced in response to JNK signaling, we examined the JAK/STAT pathway. Expression of several members of the Unpaired (Upd) family of cytokine ligands are promoted by JNK signaling (Bunker et al., 2015). The co-expression of UAS-upd1 with rnts>egr led to a dramatic increase in the frequency of ectopic wings in both wild type and CtBPQ229*/+ genetic backgrounds (Figure 6A), up to ~17% in wild type and ~90% in CtBPQ229*/+. After regeneration, the wing imaginal discs that expressed rnts>egr and >upd1 showed a high percent (85%) of large ectopic pouches (n = 13) (Figure 6B).

Figure 6 with 4 supplements see all
JAK/STAT signaling is important for the formation of the ectopic wings.

(A) Frequency of ectopic wings (EW) following rnts> driven expression of >upd1, >egr or >upd1 together with >egr in wild type and CtBPQ229*/+discs. Data were compared using ANOVA followed by Tukey test for significance (*p<0.05, **p<0.01, ***p<0.001) (B) Wing disc following rnts> driven co-expression of >egr and >upd1 after 72 hr of recovery. Pouch identity is shown by anti-Nub and an asterisk marks the ectopic pouch. (C–D) Early L3 (C) and late L3 (D) wing discs stained with anti-Wg and anti-GFP to detect the fast turnover STAT-DGFP reporter. (E–F) Wing discs with STAT-DGFP reporter following rnts>egr damage at 0 hr of recovery in wild type (E) and CtBPQ229*/+ (F) stained with anti-MMP1. Note expression of MMP1 in a subset of cells expressing STAT-DGFP in the area of ectopic pouch formation (asterisk); see (Figure 6—figure supplement 1). (G–I) Wing imaginal discs with both upd3-lacZ and STAT-DGFP reporters in undamaged (G) and damaged wild type (H) and CtBPQ229*/+ (I) discs at 0 hr of recovery. Note area in the notum that expresses STAT-DGFP but does not have elevated levels of upd3-lacZ. (J) Frequency of EW following rnts>egr damage when crossed to 1) FRT82B, 2) FRT82B Stat92E85C9, 3) FRT82B CtBPQ229*, and 4) FRT82B CtBPQ229* Stat92E85C9. Data were compared using ANOVA followed by Tukey test for significance (*p<0.05, **p<0.01, ***p<0.001). (K) Frequency of EW following rnts>egr damage in wild type and CtBP334Δ4/+ in the listed genotypes (1) +/+, (2) upd1YM55/+, (3) upd2Δ/+, (4) upd3Δ/+, and (5) upd2Δupd3Δ/+. In addition, co-expression of >upd1 with rnts>egr in (1) CtBP334Δ4/+ and (2) upd2Δupd3Δ/+;; CtBP334Δ4/+ genetic backgrounds. Note the rescue of EW induction in upd2Δupd3Δ/+ background by the co-expression of >upd1.

https://doi.org/10.7554/eLife.30391.022

During normal development, JAK/STAT signaling has been reported to occur throughout the wing imaginal disc at early stages and then becomes localized to the hinge region during L2/L3 (Ayala-Camargo et al., 2013; Hatini et al., 2013; Johnstone et al., 2013). As shown by the reporter STAT-DGFP, which encodes a destabilized GFP, the activity of JAK/STAT signaling was significantly higher in early L3 discs than late L3 discs (Figure 6C,D). After ablation of the pouch using rnts>egr in wild-type discs, STAT-DGFP expression was observed immediately surrounding the ablated pouch (Figure 6E), as observed previously, (La Fortezza et al., 2016), with very little STAT-DGFP expression in the notum. In contrast, in many CtBPQ229*/+ discs, a patch of STAT-DGFP expression was detected in the notum (Figure 6F), suggesting that JAK/STAT signaling may play a role in inducing a cell fate change. STAT-DGFP expression was often observed around sites of MMP1 expression. However, we observed that in some CtBPQ229*/+ discs, only STAT-DGFP expression was detected, without a spot of MMP1 expression, suggesting that JAK/STAT activity in the notum can occur independently of ectopic JNK activation (Figure 6—figure supplement 1).

If JAK/STAT activation occurs in the notum following damage to the pouch, where is the ligand being produced? It is known that Unpaired-family ligands are upregulated following damage to discs (Pastor-Pareja et al., 2008) and during regeneration (Katsuyama et al., 2015; Santabárbara-Ruiz et al., 2015; La Fortezza et al., 2016). We used the reporter upd3-lacZ (Bunker et al., 2015), which is not expressed at high levels in undamaged late L3 discs, to investigate where Upd3 ligand is being produced (Figure 6G). At 0 hr of recovery, upd3-lacZ expression was observed in the region of the ablated pouch in both wild type (Figure 6H) and CtBPQ229*/+ discs (Figure 6I), but not in the notum, even though STAT-DGFP expression was detected there (Figure 6I’). Since ligands of the Upd family are known to diffuse considerable distances, it is possible that the Upd ligands were generated by tissue damage and JNK activation in the pouch region and then diffused to the notum and activated JAK/STAT signaling. Indeed, the expression of UAS-upd1 in the myoblasts, which are basal to the notum epithelium, caused the activation of the JAK/STAT pathway in the notum and the disruption of the notum Wg stripe, but not the formation of an ectopic pouch (Figure 6—figure supplement 2). A similar disruption of the notum Wg stripe was observed following rnts>egr damage (Figure 3D). Thus disruption of the notum Wg stripe appears insufficient to trigger ectopic pouch formation and other events seem necessary.

If JAK/STAT activation is needed to form ectopic wings, then a decrease in JAK/STAT activity may suppress the frequency of ectopic wings. The removal of one copy of the JAK/STAT transcription factor Stat92E (FRT82B Stat92E85C9) significantly decreased the frequency of ectopic wings (EWs) when compared to FRT82B (which had a background rate of EWs) in both a wild type and CtBPQ229*/+ genetic background (Figure 6J). The reduction in the levels of the Upd-family ligands, by removal of one copy of either upd2 or upd3, or both upd2 and upd3 significantly reduced the frequency of ectopic wings (Figure 6K). In addition, this suppression was completely rescued by the addition of UAS-upd1, which indicates that the different Upd-family ligands are acting similarly in this situation. Together, this strongly indicates that the levels of JAK/STAT signaling can modulate the frequency of the notum-to-pouch cell fate change.

Does CtBP modulate the JAK/STAT pathway? First, we tested if upd3 expression was altered in CtBP-/- clones and found no change under undamaged conditions (Figure 6—figure supplement 3). Then we tested the STAT-DGFP reporter and found a slight increase in STAT signaling, although only in young discs and in regions where the pathway is normally active (Figure 6—figure supplement 4). Thus reducing CtBP levels may make tissues more responsive to the JAK/STAT pathway.

Why does the cell-fate respecification occur at a specific location in the notum?

The term ‘weak point’ has been used to describe regions prone to fate change or transdetermination, (reviewed in [McClure and Schubiger, 2007]). This might be because specific parts of the disc are more sensitive than others to the effects of Upd family ligands. Consistent with this notion, the expression of UAS-upd1 along the A-P compartment boundary specifically activated dilp8-GFP expression in the notum, in a similar location to the observed fate change in the notum (Figure 7B). In addition, this same area in the notum was specifically responsive to UAS-upd1 produced by random GAL4-expressing clones throughout the disc (Figure 7C), as shown by strong dilp8-GFP expression in this notum region (Figure 7D–F). dpp>upd1 only activated STAT-DGFP in specific regions of the notum and wing pouch, although there was an increase in apoptosis throughout the wing disc and adults showed notum defects consistent with a loss of proper notum patterning (Figure 7—figure supplement 1). Taken together, these experiments indicate that there is a region in the notum of the wing disc that is specifically and highly responsive to Upd ligands. However, the addition of UAS-upd1 without activation of JNK did not seem to be sufficient to trigger a fate change suggesting that JNK signaling and JAK/STAT signaling function together to promote re-specification of cell fates.

Figure 7 with 1 supplement see all
‘Weak point’ in the wing imaginal disc is responsive to Upd1 ligand and model for notum to wing transdetermination.

(A, B) Wing discs with dilp8-GFP and vgQE-RFP reporters: control (A), and dpp-GAL4, UAS-upd1 (B). Note the specific expression of dilp8-GFP along the posterior edge of the notum and in the wing pouch (arrows). (C) Overexpression of UAS-upd1 by heat-shock induced flip-out clones (hs-FLP, Act<stop<GAL4) marked with UAS-RFP. Note the specific area in the notum that responds to Upd1 by expressing dilp8-GFP (arrows). (D) Model for how JAK/STAT and JNK/AP-1 signaling work together to trigger a fate change and the growth of an ectopic pouch. Damage to the normal wing pouch generates both Egr and Upd ligands. The weak point, an area near the anterior/posterior compartment boundary in the notum responds to Upd ligands and the resulting JAK/STAT signaling disrupts the normal notum identity (as observed with the disruption of the notum Wg stripe). JNK activity within a field of JAK/STAT activity leads to the expression of Wg, which triggers cells to adopt the new wing pouch fate. Then, as in the regenerating wing pouch, additional cells are recruited to generate a new pouch. CtBP functions, either directly or indirectly, to antagonize these pathways.

https://doi.org/10.7554/eLife.30391.027

Discussion

The replacement of damaged tissue by the proliferation of adjacent cells requires those cells to change fates, often in subtle ways. In the imaginal disc, cells at each location have distinct patterns of gene expression. Hence, if portions of the disc are eliminated and replaced by the proliferation of nearby cells, the newly generated cells will need to adopt characteristics distinct from the cells that they are derived from. At the same time, other cells need to preserve established patterns of gene expression. Our work suggests that the limited plasticity that is necessary for regeneration results from an interplay of pathways that promote plasticity such as JNK/AP-1 and JAK/STAT with regulators that limit the activity of these pathways such as CtBP.

The relationship between ablation of the pouch and activation of the JNK/AP-1 and JAK/STAT in the notum

Activation of two pathways, JNK/AP-1 and JAK/STAT, appears to be necessary for promoting cells in the notum to adopt a pouch fate. How does ablation of the pouch promote the activation of these pathways in the notum? Neither ablation of the pouch using rpr nor activation of the Egr-receptor Grind in the pouch suffices. Thus, Egr is necessary and it either activates additional Grnd-independent pathways, or, more likely, activation of the Egr pathway in cells outside the rn-GAL4 expression domain is necessary. This could be both to activate JNK/AP-1 signaling locally around the damaged pouch and at a greater distance in the notum. The local signal to the hinge cells surrounding the wing pouch may produce the upd ligands, as these cells normally express upd1. Egr may also signal directly to the notum, as a cleaved secreted ligand or from membrane fragments of cellular debris, much of which is trapped apically. In support of this idea, a secreted form of Egr is more effective than the membrane tethered form at inducing ectopic wings. Since reducing CtBP function increases AP-1 activity, the notum of CtBP-/+ discs will likely be more responsive to Egr signaling, leading to the activation of downstream AP-1 targets, such as dilp8 and wg.

STAT-DGFP expression in the notum is increased in CtBP heterozygotes following ablation of the pouch. Increased JNK activity in the dying cells of the pouch would be expected to generate increasing levels of Upd-family ligands since they are upregulated in regenerating discs (Katsuyama et al., 2015; Santabárbara-Ruiz et al., 2015; La Fortezza et al., 2016) and regulatory elements of these genes have AP-1-binding sites (Bunker et al., 2015). Consistent with their production by dying cells is the observation that more rapid killing of pouch cells by co-expression of rpr reduces notum-to-pouch transformations.

Increased STAT activity in the notum reduces notum-specific patterns of gene expression and promotes a hinge-like fate (Ayala-Camargo et al., 2013). Consistent with this, we found that reducing gene dosage of mirr, a homeodomain-containing protein expressed in the notum, increased the frequency of ectopic wings. A recent study reported the generation of ectopic wings simply by expression of UAS-upd1 in the notum (without directed tissue damage) (Recasens-Alvarez et al., 2017). However, this study induced expression in the second larval instar (day 5 at 18°C) and did not report if expression of UAS-upd1 at later time points could also induce ectopic wings. Of note, we have found that expression of high levels of UAS-upd1 generates considerable levels of apoptosis. Conceivably, the generation of ectopic wings in that report could therefore also have resulted from the combined activation of the JAK/STAT and AP-1 pathways.

Why does formation of the ectopic pouch begin at a specific location in the notum?

Imaginal discs have been hypothesized to have ‘weak points’, where transdetermination occurs most often following physical fragmentation (Schubiger, 1971), (reviewed in [McClure and Schubiger, 2007]). Other cell fate transformations are also more likely to occur in particular regions of the discs (Salzer and Kumar, 2010). For leg-to-wing transdetermination in the prothoracic leg disc, the weak point is located where two different morphogens, Wg and Dpp, are co-expressed (Johnston and Schubiger, 1996; Maves and Schubiger, 1998). In the wing disc, Dpp is expressed along the anteroposterior (AP) compartment boundary and Wg, is expressed along part of the dorsoventral (DV) compartment boundary through the wing pouch. The AP and DV boundaries likely intersect at two locations – one in the middle of the wing pouch and in the notum near the region where we observe ectopic pouch formation. In addition, the notum Wg stripe in the L3 disc generates an additional location where both Wg and Dpp are expressed. Therefore, it is possible that similar to the weak point in the leg disc, the presence of both these morphogens makes cells more prone to change fate, especially following damage.

This region of the notum could be predisposed to an increase in STAT activity. When UAS-upd1 is expressed using dpp-GAL4, STAT-DGFP expression is not observed along the entire GAL4 domain. Rather, it is mostly restricted to the pouch, and importantly, a region of the notum. These regions are more responsive to Upd-family ligands than other parts of the disc and the area in the notum is likely the weak point for notum-to-pouch fate change. Recent studies have described regions in wing discs that are tumor hot-spots (Tamori et al., 2016) and are resistant to apoptosis (Verghese and Su, 2016) and found that they also have elevated JAK/STAT activity. Thus, parts of the disc that have elevated STAT activity may be more capable of surviving damage and then re-specifying cell fates.

Events during the formation of an ectopic pouch have similarities to specification of the pouch during normal development

During normal development, the initial specification of the wing pouch occurs towards the end of the first larval instar. At this time STAT is active through most of the wing disc and wg is expressed in a patch in the anterior and ventral portion of the disc. Subsequently, wg expression expands from its initial region of expression when cells surrounding the nascent pouch are recruited to a pouch fate by a feed-forward mechanism that is fueled by Wg (Wu and Cohen, 2002; Zecca and Struhl, 2007b, 2010). In the absence of Wg expression, the pouch is not specified.

In our system, wg expression from the damage-responsive enhancer is important for triggering ectopic wings. However, we found that additional Wg (rnts>egr, >wg), if at all, decreased the frequency of ectopic wings and that Wg alone was incapable of transforming a more mature notum to an ectopic pouch; therefore JAK/STAT and AP-1 activity appear necessary. Based on our observations and those of others, JAK/STAT activity can reduce the expression of notum-specific genes (Ayala-Camargo et al., 2013). This likely transforms that part of the notum to a less committed state. Thus, a region with elevated STAT activity leads to relatively uncommitted notum cells and within this region, the activation of AP-1 promotes Wg expression via a damage-responsive enhancer, which may create conditions similar to the initial specification of the wing pouch at earlier stages of development (Figure 7D).

Once the ectopic pouch has been specified, the nascent pouch could turn on the rn-GAL4 driver, even briefly, prior to the downshift. Then egr expression would occur resulting in localized apoptosis and JNK activation. The surrounding cells would activate AP-1 and STAT and also express wg as occurs in the regeneration blastema surrounding rnts>egr ablated tissue. This would then have the effect of reinforcing the conditions that are necessary for notum-to-pouch fate change and the generation of a new wing pouch. While this paper was under review, another paper was published that gives support to damage-induced fate changes relying on JAK/STAT and Wg signaling (Verghese and Su, 2017).

Role of CtBP in resisting cell fate changes

We have shown that clones of cells lacking CtBP function have elevated levels of AP-1 activity and, in a few cases in specific portions of the disc, increased STAT activity. CtBP is a co-repressor that interacts with a number of transcriptional repressors via a PxDLS motif including Brinker (Hasson et al., 2001) and Hairy (Poortinga et al., 1998) and hence multiple CtBP-containing complexes could be relevant for this role of CtBP. Intriguingly, some of the isoforms of the Drosophila Fos ortholog, Kayak, which heterodimerizes with Jun to form the AP-1 transcription factor, have PxDLS motifs. While AP-1 has mostly been studied as a transcription factor that activates gene expression upon phosphorylation of Jun by JNK, in the absence of sufficient activating signals, it may repress inappropriate expression of AP-1 target genes via CtBP. In this way, CtBP could buffer cell fates from destabilization caused by fluctuations in the level of JNK activity.

Materials and methods

Fly stocks

The stocks that were used in this study include: rn-GAL4, tub-GAL80ts, rn-GAL4, tub-GAL80ts, UAS-egr and rn-GAL4, tub-GAL80ts, UAS-rpr (Smith-Bolton et al., 2009), hh-GAL4, ptc-GAL4, tub-GAL80ts, nub-GAL4; tub-GAL80ts, UAS-egr/TM6B-GAL80, dpp-GAL4 (BL:1553), R15B03-GAL4 (BL:49261), R76A01-GAL4 (BL:46953) (Pfeiffer et al., 2008), G-TRACE (BL:28280, BL:28281) and Ubi<stop<GFPnls (BL:32250, BL:32251)(Evans et al., 2009), Act5C>FRT.CD2>GAL4, UAS-RFP (BL:30558), vgQE-RFP (Zecca and Struhl, 2007a), hs-FLP; Act<stop<lacZnls, Ubi<stop<GFPnls (Worley et al., 2013), UAS-CtBP (Bhambhani et al., 2011), Genomic CtBP construct (gCtBP) (Zhang and Arnosti, 2011), UAS-ecto-eiger (Narasimamurthy et al., 2009), UAS-grindICD (Andersen et al., 2015), MMP1-LacZ (Uhlirova and Bohmann, 2006), AP-1-GFP and AP-1-RFP reporters (Chatterjee and Bohmann, 2012), upd3-lacZ (Bunker et al., 2015), upd3.1-lacZ (Jiang et al., 2011), BRV-B-GFP (Harris et al., 2016), UAS-DroncDN (UAS-DroncC318S)(Hawkins et al., 2000), FRT82B, FRT82B CtBPQ229* and FRT82B Stat92E85C9. Stocks obtained from Bloomington stock center include: CtBP87De-10 (BL:1663), CtBP03463 (BL:11590), UAS-CtBPRNAi (BL:31334, BL:32889), mirr1486 (BL:23935), mirr1825 (BL:23928), hepr75 (BL:6761), UAS-FosDN (UAS-Fra.Fbz, BL:7214), UAS-JNKDN (UAS-bskK53R, BL:9311), UAS-p35 (BL:5072, 5073), dIlp8MI00727 (BL:33079), UAS-wg (BL:5918, BL:5919), UAS-hepCA (BL:6406), lexAOp-FLP (BL:55820), R81E08-lexA (BL:54377), R76B02-lexA (BL:54118), R76B06-lexA (BL:54225), R15C03-lexA (BL:52490), 10XSTAT92E-GFP (BL:26197) and 10XSTAT92E-DGFP (BL:26199) (Bach et al., 2007), Df(3R)Exel8157 (BL:7973), and upd2Δ (BL:55727), upd2Δupd3Δ (BL:55729), upd3Δ (BL:55728)(Osman et al., 2012).

Temperature shift and clone induction experiments

Genetic ablation experiments were conducted as described in (Smith-Bolton et al., 2009). Briefly, eggs were collected on grape plates and animals were density controlled by picking 55 L1 larvae into vials with yeast paste. Shifts were conducted on particular days (day 3 - day 9) AEL from an 18°C incubator to 30°C incubator. Cultures were shifted on day 7 AEL for 40 hr unless otherwise noted. Experimental replicates were done on separate days. Adults were scored as (1) No EW for no ectopic wings or (2) EW for either one or two ectopic wings, except in (Figure 3), where adults were scored for having zero, one, or two ectopic wing(s). Graphs show average frequency of EWs for experiments done on separate days. Error bars show standard deviations between the experiments.

To generate CtBP mutant clones, hs-FLP;;FRT82B RFPnls was crossed to FRT82B CtBPQ229* and vials were heat shocked at 37°C for 1 hr to induce mitotic clones. To generate randomly marked clones, hs-FLP;;rnts>egr/TM6B, Tub-GAL80 was crossed to Act5C<stop<lacZnls, Ubi<stop<GFPnls; CtBPQ229*/TM6B and the cultures were staged as described above. A brief 10 min 37°C heat-shock was used to generate flip-out clones at a relatively low density. Without a 37°C heat shock, the 30°C temperature shift for the genetic ablation experiments did not produce hs-FLP induced clones, which we also noted in (Smith-Bolton et al., 2009).

Immunohistochemistry

Imaginal discs were fixed in 4% paraformaldehyde for 15 min, washed and permeabilized in phosphate-buffered saline solution with 0.1% Triton X-100, and blocked in either 10% Normal Goat Serum or Normal Donkey Serum depending on staining. The following antibodies were used from Developmental Studies Hybridoma Bank (DSHB): mouse anti-Wg (1:100, 4D4); mouse anti-Mmp1 (1:100, a combination of 14A3D2, 3A6B4 and 5H7B11); mouse anti-En (1:10, 4D9); rat anti-Ci (1:10, 2A1); mouse anti-Cut (1:200, 2B10); mouse anti-Ptc (1:50, Apa-1); and mouse anti-Ubx (1:20, FP3.38). The following antibodies were gifted: rat anti-Pdm2 (Chris Doe); rat anti-Twist (1:1000, Eric Wieschaus); and mouse anti-Nub and rabbit anti-Tsh (Stephen Cohen). The following antibodies are from commercial sources: goat anti-dCtBP (1:50, dN-20 Santa Cruz Biotechnology, Dallas TX); rabbit anti-DCP-1 (1:250, Cell signaling); rabbit anti-GFP (1:500, Torrey Pines Laboratories, Secaucus, NJ); chicken anti-GFP (1:500, ab13970 Abcam, Cambridge, UK); and rabbit anti-β-galactosidase (1:1000, #559762; MP Biomedicals, Santa Ana, CA). Secondary antibodies were from Cell Signaling. Nuclear staining was by DAPI (1:1000, Cell Signaling). Images were obtained on either a Leica TCS or a Zeiss LSM 700. Images were processed using ImageJ (Fiji) (Schindelin et al., 2012). All scale bars are 100 μm.

For scoring discs with dilp8-GFP expression in the notum or ectopic pouch at different time points of recovery, in (Figure 3), images were collected from discs from biological replicates (cultures started on separate days) and imaged on Zeiss Axio Imager M1 without staining with anti-GFP. Images were collected and then scored for the presence or absence of a second spot of dilp8-GFP expression.

Generation of CtBP CRISPR alleles

We generated CRISPR guide RNAs to regions conserved in all CtBP isoforms, using the method described in FlyCas9 system (Kondo and Ueda, 2013). We generated stable transgenetics using the U6-promoter driving the guide RNAs inserted at the attP40 landing site.The guide RNAs were optimized to work in our wtiso genetic background, as we sequenced the predicted regions guide RNA binding, detected single nucleotide polymorphisms as compared to the FlyBase consensus, and incorporated these changes into the guide RNA sequence. We used the transgenic services provided by BestGene (Chino Hills, CA). We generated the following stocks to generate CRISPR mutations on particular third chromosomes: Sp/Cyo, nos-Cas9; wtiso and Sp/Cyo, nos-Cas9; rn-GAL4, UAS-eiger, tub-GAL80ts, which were crossed to U6-CtBP-guideRNA; TM2/TM6B in order to recover CRISPR generated mutations on particular third chromosomes. Single males carrying possible CtBP alleles were tested for the failure to complement viability when crossed to a deletion that spans the CtBP gene, Df(3R)Exel8157. The newly generated CtBP alleles were then sequenced to determine the nucleotide change near the guide RNA cut site.

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Decision letter

  1. Bruce Edgar
    Reviewing Editor; University of Utah, United States

In the interests of transparency, eLife includes the editorial decision letter and accompanying author responses. A lightly edited version of the letter sent to the authors after peer review is shown, indicating the most substantive concerns; minor comments are not usually included.

Thank you for submitting your article "The transcriptional co-repressor CtBP impedes cell fate misspecifications in regenerating Drosophila imaginal discs" for consideration by eLife. Your article has been reviewed by three peer reviewers, one of whom, Bruce Edgar (Reviewer #1), is a member of our Board of Reviewing Editors, and the evaluation has been overseen by Didier Stainier as the Senior Editor. The following individuals involved in review of your submission have agreed to reveal their identity: Giovanni Bosco (Reviewer #3).

The reviewers have discussed the reviews with one another and the Reviewing Editor has drafted this decision to help you prepare a revised submission.

Reviewing Editor's comments:

All three reviewers appreciated the approaches used in this paper, and its content. However reviewer #1 felt that the paper was much too long and had many inconclusive sections that could be condensed or removed. In discussions, the other reviewers agreed with this perspective.

Reviewer #3 also felt that the paper should have delivered more mechanistic insight as to how CtBP affects transdetermination, but we understand that providing this could be challenging and time-consuming, and so we decided that it is not required at this stage. Hence we would like to invite you to submit a revised manuscript that is significantly shorter than the current version (30-50%) and more linear in presentation. Specific suggestions for how to do this can be found in the reviews, which I include below essentially in their entirety.

In addition, the points #4 and #6 from reviewer 1 merit special consideration – if you can provide further data addressing these points this would be much appreciated. At the very least, a clear discussion of the action of egr is needed. The reviewers also had a number of minor comments regarding controls, clarification of methods and interpretation of the results, which you should address in your revision. Overall we agreed that the paper was sufficiently developed and could be published without large amounts of additional data, provided the delivery is succinct and clear. eLife looks forward to receiving your revision.

Reviewer #1:

In this paper, Worley, Alexander, and Hariharan revisit the phenomenon of damage-initiated trans-determination in Drosophila wing imaginal discs, using new genetic methods to identify the genes involved. This is an interesting process with potentially broad relevance, but little progress has been made on it in years. The authors present a very nice genetic saturation screen of the third chromosome (~40% of the genome) that identifies many genes potentially involved. Then they focus on one gene, CtBP at 87D, and show how this affects transdetermination of notum cells to wing pouch cells. The process involves JNK and STAT activation (as expected) at the wound site, is multi clonal, and involves the activation of a number of other genes that are tracked. The effects of these genes are are clearly demonstrated, but the paper falls short of determining any clear mechanisms at the molecular level.

This manuscript starts out nicely with one of the best introductions on the subject of transdetermination that I've read, and succinct descriptions of the damage protocol (already detailed in a previous publication) and the modifier screen, which is clever and effective (Figure 1). The effect of CtBP is clear, but it was not obvious why the authors focused on this one gene, and this should be stated. Following this nice entry, the paper details a huge number of genetic tests of mechanism in the subsequent 7 figures and 15 pages of meandering text. The specific tests that were done are all logical, and the results are interpreted in a critical fashion, but unfortunately they don't come together in a very readable, coherent form. Although the effects of egr, Ap1, Stat, etc are clear, the authors don't succeed in demonstrating how these factors work together very well, and some obvious questions are left unresolved (see below). In addition, many tests that were relatively inconclusive are presented, as well as quite a few negative results and dead ends. Many paragraphs in the Results section don't have a conclusion at all. Overall the Results section meanders from one issue to the next, with too much discussion, and no obvious direction. It is far too long. It seems to be a very raw draft of a large body of work, essentially un-refined, and it really should be re-written in a much more concise, linear format to be digestible by a general audience. Much of what is here could probably be presented much more simply, or just omitted, without affecting the paper's final conclusions. I suggest trying to pare it down to about half the current length. While I think the core content of this paper is valuable and should be published, I cannot recommend it in its current form. Specific points follow below:

1) There is a long section about the Rga locus but then this locus is never mentioned again. What is it's map location? What is its relevance to the paper's overall conclusion? This locus justifies the screen, but if it is not relevant to the paper's conclusions the section devoted to it should be removed. The paper contains several other examples of discussion of this sort of irrelevant, distracting data.

2) The authors should note why they focused on region 87D after doing the screen. Further discussion of other loci that strongly affected transdetermination could enhance this paper, if the genes involved are known. Nevertheless, it is very nice that the authors include the complete results of their very elegant screen (Figure 1I, Supplementary File 1).

3) The long paragraph in subsection “Re-specifying cell fates requires the activation of the JNK/AP-1 pathway” is an example of a discussion of results that meanders and has no conclusion.

4) There are quite a few experiments that address the requirements of egr, Jnk, and apoptosis in promoting transdetermination, and much discussion about this. However the paper doesn't seem to have a clear conclusion about whether egr triggers transdetermination via JNK-mediated AP1 activation, or JNK-mediated apoptosis, or both. Egr is clearly sufficient, and JNK required but not sufficient, and apoptosis is not sufficient, but it's not clear what, downstream of egr, is doing it. Is apoptosis required? I think a few more experiments are required here, and a cleaner more definitive conclusion is needed about which downstream targets of egr are critical.

5) The effects on dILP8 expression are interesting and suggestive (“dilp8 expression in a secondary location is predictive of ectopic wing pouch formation”), but dILP8 function is not tested. It would be a nice addition to the paper if the role of dILP8 were tested using mutants, RNAi, and overexpression.

6) Upd ligand production, in response to egr, or Ap1, or apoptosis directly, seems to be an important aspect of the authors proposed mechanism (Figure 8Q, and Results). However they don't seem to have tested the requirement functionally, except by Upd1 overexpression and in Stat+/- mutants. There are upd2, upd3, and upd2,3 deletion lines that are viable and could be used to test the requirement of these damage-dependent ligands.

7) Given the multitude of tests presented, the summary diagram (Figure 8Q) is surprisingly simple. Could the authors add more detail to this? Alternatively, the paper could be much more readable if it included ONLY results that are directly relevant to this model.

Reviewer #2:

The manuscript by Worley et al. shows the requirement of the transcriptional co-repressor CtBP for proper cell fate specifications in regenerating Drosophila larval wing imaginal discs after apoptosis-induced damage. The authors first find that, in certain genetic backgrounds, regeneration after rnts>egr damage produces ectopic wing tissues. They then conduct a genetic screen using stocks bearing deletions of the third chromosome in the rnts>egr background and find that many deletions induce the formation of ectopic wings at varied penetrance. They then identify and focus on CtBP, a transcriptional co-repressor. Regarding the signaling pathway, the authors demonstrate that Egr-dependent JNK activation in the wing pouch is necessary for the generation of ectopic wings and that JAK-STAT signaling promotes the notum-to-pouch transformation. They further find that cells in the notum are re-specified to ectopic wing pouch, but maintain their compartment identity, show that epigenetic regulation plays an opposite role to STAT and Wg in modulating the frequency of ectopic growth. They finally show that loss of CtBP increases the AP-1 activity and propose a model to explain how CtBP prevents cell fate specifications in regenerating Drosophila imaginal discs.

The results presented in this manuscript are very interesting and will be of interest to the field of tissue regeneration and developmental signaling. The authors conduct a series of elegant genetic assays and provide compelling results to validate the conclusions they made, therefore the conclusions are convincing.

Specific Comments:

1) Figure 4K. Since temperature shift and genetic background affect the frequency of ectopic wings, in order to conclude that "expression of >egr in the wing pouch is the major cause of generating ectopic wings", the authors also need to test the R15B03-, R76A01-, and dpp-Gal4 drivers using the same temperature shift protocol.

2) Scale bar is missing in some figures.

3) Since the clean genetic background did not produce ectopic wings in rnts>egr, the description at the beginning part of the manuscript is misleading. This information should be included in the Abstract.

4) rnts control is needed for Figure 2—figure supplement 1A.

5) G-trace with low- and high-flp needs to be better described in the text/(Figure 3—figure supplement 1).

6) Figure 8A-H, MMP1-lacZ is robustly upregulated in CtBP homozygous mutant clones, whereas, AP-1-GFP is only found in a few cells of CtBP mutant clones. What causes the dramatic difference of these two JNK signaling reporters upon CtBP loss?

Reviewer #3:

The manuscript by Worley and colleagues seeks to understand mechanisms of cellular reprogramming during tissue regeneration while keeping in check inappropriate cell fates and proliferation. The authors use the Drosophila wing disc as a model of regeneration after induced cell death in order to screen for factors that modify the formation of regenerated wings and wing tissue. This genetics screen reveals that the C-terminal Binding Protein (CtBP) likely inhibits changes in cell fates and limits inappropriate differentiation and proliferation. Through a series of tenacious and elegant genetic experiments the authors show that a combination of JAK/STAT activation and AP-1 activity cell specifically located at the "weak point" of the wing disc notum can switch cell fates when triggered to regenerate after tissue damage. Reduction of CtBP function (either in a heterozygous background or homozygous clones) increases AP-1, as assayed by an AP-1-GFP reporter and is proposed to increase the levels of cell fate changes. Although it is not clear how CtBP modulates AP-1 levels and/or what other CtBP target genes contribute to restricting cell fate changes, these observations are interesting in and of themselves as they lay the foundation upon which more molecular mechanistic experiments can be done. For example, what exactly constitutes "weak points", how does CtBP co-repressor work to modulate AP-1 activity specifically at the proposed weak point, and consequently are Upd-family ligands directly involved in cell fate determination in the context of regenerating tissue? Although this study identifies CtBP as a previously unrecognized modulator of cellular plasticity, it remains unclear how it achieves this and how much more molecular mechanism could/should have been elucidated. Other than that I do not have substantive concerns.

https://doi.org/10.7554/eLife.30391.032

Author response

Reviewing Editor's comments:

All three reviewers appreciated the approaches used in this paper, and its content. However reviewer #1 felt that the paper was much too long and had many inconclusive sections that could be condensed or removed. In discussions, the other reviewers agreed with this perspective.

Reviewer #3 also felt that the paper should have delivered more mechanistic insight as to how CtBP affects transdetermination, but we understand that providing this could be challenging and time-consuming, and so we decided that it is not required at this stage. Hence we would like to invite you to submit a revised manuscript that is significantly shorter than the current version (30-50%) and more linear in presentation. Specific suggestions for how to do this can be found in the reviews, which I include below essentially in their entirety.

Thank you for the opportunity to revise the manuscript. We have rewritten the manuscript completely. The Introduction and Results and Discussion section is now 30% shorter. Importantly we feel that the logical flow is much improved. We took three months (rather than the two months you suggested) because some of the additional experiments took a bit longer (One generation in our ablation/regeneration system takes 22-25 days).

In addition, the points #4 and #6 from reviewer 1 merit special consideration – if you can provide further data addressing these points this would be much appreciated. At the very least, a clear discussion of the action of egr is needed. The reviewers also had a number of minor comments regarding controls, clarification of methods and interpretation of the results, which you should address in your revision. Overall we agreed that the paper was sufficiently developed and could be published without large amounts of additional data, provided the delivery is succinct and clear. eLife looks forward to receiving your revision.

We have included additional data on the action of eiger (as detailed in responses below to specific reviewer comments).

Reviewer #1:

In this paper, Worley, Alexander, and Hariharan revisit the phenomenon of damage-initiated trans-determination in Drosophila wing imaginal discs, using new genetic methods to identify the genes involved. This is an interesting process with potentially broad relevance, but little progress has been made on it in years. The authors present a very nice genetic saturation screen of the third chromosome (~40% of the genome) that identifies many genes potentially involved. Then they focus on one gene, CtBP at 87D, and show how this affects transdetermination of notum cells to wing pouch cells. The process involves JNK and STAT activation (as expected) at the wound site, is multi clonal, and involves the activation of a number of other genes that are tracked. The effects of these genes are are clearly demonstrated, but the paper falls short of determining any clear mechanisms at the molecular level.

This manuscript starts out nicely with one of the best introductions on the subject of transdetermination that I've read, and succinct descriptions of the damage protocol (already detailed in a previous publication) and the modifier screen, which is clever and effective (Figure 1). The effect of CtBP is clear, but it was not obvious why the authors focused on this one gene, and this should be stated. Following this nice entry, the paper details a huge number of genetic tests of mechanism in the subsequent 7 figures and 15 pages of meandering text. The specific tests that were done are all logical, and the results are interpreted in a critical fashion, but unfortunately they don't come together in a very readable, coherent form. Although the effects of egr, Ap1, Stat, etc are clear, the authors don't succeed in demonstrating how these factors work together very well, and some obvious questions are left unresolved (see below). In addition, many tests that were relatively inconclusive are presented, as well as quite a few negative results and dead ends. Many paragraphs in the Results section don't have a conclusion at all. Overall the Results section meanders from one issue to the next, with too much discussion, and no obvious direction. It is far too long. It seems to be a very raw draft of a large body of work, essentially un-refined, and it really should be re-written in a much more concise, linear format to be digestible by a general audience. Much of what is here could probably be presented much more simply, or just omitted, without affecting the paper's final conclusions. I suggest trying to pare it down to about half the current length. While I think the core content of this paper is valuable and should be published, I cannot recommend it in its current form. Specific points follow below:

We have put a lot of effort in re-writing the manuscript. It is much shorter, and we think it now has a clear logical flow. We have removed sections that add little to our final conclusions.

1) There is a long section about the Rga locus but then this locus is never mentioned again. What is it's map location? What is it's relevance to the paper's overall conclusion? This locus justifies the screen, but if it is not relevant to the paper's conclusions the section devoted to it should be removed. The paper contains several other examples of discussion of this sort of irrelevant, distracting data.

We have removed the section on the Rga locus since it is not particularly relevant to the overall conclusions of our study.

2) The authors should note why they focused on region 87D after doing the screen. Further discussion of other loci that strongly affected transdetermination could enhance this paper, if the genes involved are known. Nevertheless, it is very nice that the authors include the complete results of their very elegant screen (Figure 1I, Supplementary file 1).

The reason we focused on 87D was because this is the only region thus far, where we have been able to unambiguously identify the gene within the deletion, that when mutated, robustly enhanced the frequency of notum-to-pouch fate change. We did include all the data from our deficiency screen so others could use our data to explore candidate genes if they wish.

3) The long paragraph in subsection “Re-specifying cell fates requires the activation of the JNK/AP-1 pathway” is an example of a discussion of results that meanders and has no conclusion.

We have eliminated this and other similar paragraphs.

4) There are quite a few experiments that address the requirements of egr, Jnk, and apoptosis in promoting transdetermination, and much discussion about this. However the paper doesn't seem to have a clear conclusion about whether egr triggers transdetermination via JNK-mediated AP1 activation, or JNK-mediated apoptosis, or both. Egr is clearly sufficient, and JNK required but not sufficient, and apoptosis is not sufficient, but it's not clear what, downstream of egr, is doing it. Is apoptosis required? I think a few more experiments are required here, and a cleaner more definitive conclusion is needed about which downstream targets of egr are critical.

We have included additional data that address these issues. Our experiments show that apoptosis of the pouch, in itself does not promote the notum-to-pouch transformation. Ablation with reaper does not cause ectopic pouch formation nor does hastening death by co-expressing eiger and reaper. Our data suggest that cells with high levels of AP-1 activation, express target genes such as unpaired-family genes and dilp8 which contribute to the fate change. We also show that strictly cell autonomous activation of Eiger signaling in the pouch does not suffice. It is possible that this is because cells in the hinge are more capable of expressing high levels of Upd-family proteins than cells in the pouch and do so when they are exposed to Eiger.

5) The effects on dILP8 expression are interesting and suggestive (“dilp8 expression in a secondary location is predictive of ectopic wing pouch formation”), but dILP8 function is not tested. It would be a nice addition to the paper if the role of dILP8 were tested using mutants, RNAi, and overexpression.

Thank you for this suggestion. We have included additional data that show that reducing dilp8 function reduces the frequency of ectopic pouches and increasing dilp8 expression increases the frequency.

6) Upd ligand production, in response to egr, or Ap1, or apoptosis directly, seems to be an important aspect of the authors proposed mechanism (Figure 8Q, and Results). However they don't seem to have tested the requirement functionally, except by Upd1 overexpression and in Stat+/- mutants. There are upd2, upd3, and upd2,3 deletion lines that are viable and could be used to test the requirement of these damage-dependent ligands.

We have now included these experiments. The upd 2,3 deletion dominantly reduces the frequency of ectopic pouches and this effect is overcome by co-expression of upd1. These experiments show that upd 2 and 3 are necessary for ectopic pouch formation and that the different upd family members can function interchangeably in this situation. This strengthens our argument that signaling from the damaged wing pouch to the notum is important for triggering this fate change.

Reviewer #2:

[…]

Specific Comments:

1) Figure 4K. Since temperature shift and genetic background affect the frequency of ectopic wings, in order to conclude that "expression of >egr in the wing pouch is the major cause of generating ectopic wings", the authors also need to test the R15B03-, R76A01-, and dpp-Gal4 drivers using the same temperature shift protocol.

We conducted these experiments with tub-GAL80ts and the same temperature shift protocol. We did not observe ectopic wings. The data are shown in (Figure 5—figure supplement 3).

2) Scale bar is missing in some figures.

We have added scale bars to all of the main figures and to most of the figure supplements.

3) Since the clean genetic background did not produce ectopic wings in rnts>egr, the description at the beginning part of the manuscript is misleading. This information should be included in the Abstract.

We have changed the relevant sentence in the Abstract to be more specific:

“As a result of this screen, we found that reducing function of the transcriptional co-repressor C-terminal Binding Protein (CtBP) results in an increased frequency of inappropriate changes in cell fate.”

has been changed to

“As a result of this screen, we found that reducing function of the transcriptional co-repressor C-terminal Binding Protein (CtBP) results in inappropriate changes in cell fate, which are not observed in wild type.”

4) rnts control is needed for Figure 2—figure supplement 1A.

We have added the non-ablated controls in Figure 2 and Figure 2—figure supplement 1A.

5) G-trace with low- and high-flp needs to be better described in the text/(Figure 3—figure supplement 1).

We have re-written this portion of the text to be clearer.

6) Figure 8A-H, MMP1-lacZ is robustly upregulated in CtBP homozygous mutant clones, whereas, AP-1-GFP is only found in a few cells of CtBP mutant clones. What causes the dramatic difference of these two JNK signaling reporters upon CtBP loss?

We have consistently observed a “boundary effect” with the AP-1-GFP reporter, which we also observe with dilp8-GFP. We have no good explanation for this phenomenon. The MMP1-lacZ reporter appears to have a basal level of expression levels throughout the disc, and may also contain an enhancer that is more responsive to the loss of CtBP. Note that we do not detect MMP1 protein in CtBP-/- mutant clones and therefore the MMP1-lacZ reporter is active but not the endogenous gene. In addition, MMP1-lacZ reporter expression was detected with an antibody, which may detect β-GAL produced over a longer time window, while both AP-1-GFP and dilp8-GFP were observed without an antibody. This could account for some of the differences.

https://doi.org/10.7554/eLife.30391.033

Article and author information

Author details

  1. Melanie I Worley

    Department of Molecular and Cell Biology, University of California, Berkeley, Berkeley, United States
    Contribution
    Conceptualization, Data curation, Formal analysis, Supervision, Validation, Investigation, Visualization, Methodology, Writing—original draft, Writing—review and editing
    Competing interests
    No competing interests declared
    ORCID icon 0000-0001-9772-4985
  2. Larissa A Alexander

    Department of Molecular and Cell Biology, University of California, Berkeley, Berkeley, United States
    Contribution
    Data curation, Investigation
    Competing interests
    No competing interests declared
  3. Iswar K Hariharan

    Department of Molecular and Cell Biology, University of California, Berkeley, Berkeley, United States
    Contribution
    Conceptualization, Supervision, Funding acquisition, Writing—original draft, Project administration, Writing—review and editing
    For correspondence
    ikh@berkeley.edu
    Competing interests
    No competing interests declared
    ORCID icon 0000-0001-6505-0744

Funding

National Institute of General Medical Sciences (GM061672)

  • Iswar K Hariharan

American Cancer Society (RP-16-238-06-COUN)

  • Iswar K Hariharan

National Institute of General Medical Sciences (GM085576)

  • Iswar K Hariharan

National Institute of General Medical Sciences (GM122490)

  • Iswar K Hariharan

The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.

Acknowledgements

The authors would like to thank D Arnosti, E Bach, K Basler, K Cadigan, C Doe, S Cohen, P Leopold, G Struhl, E Wieschaus, and M Zeidler for stocks and reagents. We thank current and former members of the Hariharan lab for useful feedback, especially T Sumabat and L Setiawan. We thank D Bilder and the Bilder lab members for advice. We thank E Bondra, K Gandhi, and V Dhruva for technical assistance. We thank the Bloomington Stock Center, Drosophila Genomics Resource Center, Developmental Studies Hybridoma Bank, and BestGene for stocks, reagents, and services. This work was funded by NIH grants R01 GM061672, R01 GM085576, and R35 GM122490 and a Research Professor Award from the American Cancer Society (RP-16238–06-COUN).

Reviewing Editor

  1. Bruce Edgar, Reviewing Editor, University of Utah, United States

Publication history

  1. Received: July 13, 2017
  2. Accepted: January 19, 2018
  3. Accepted Manuscript published: January 26, 2018 (version 1)
  4. Version of Record published: February 22, 2018 (version 2)

Copyright

© 2018, Worley et al.

This article is distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use and redistribution provided that the original author and source are credited.

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