The Hippo signalling pathway restricts cell proliferation in animal tissues by inhibiting Yes-associated protein (YAP or YAP1) and Transcriptional Activator with a PDZ domain (TAZ or WW-domain–containing transcriptional activator [WWTR1]), coactivators of the Scalloped (Sd or TEAD) DNA-binding transcription factor. Drosophila has a single YAP/TAZ homolog named Yorkie (Yki) that is regulated by Hippo pathway signalling in response to epithelial polarity and tissue mechanics during development. Here, we show that Yki translocates to the nucleus to drive Sd-mediated cell proliferation in the ovarian follicle cell epithelium in response to mechanical stretching caused by the growth of the germline. Importantly, mechanically induced Yki nuclear localisation also requires nutritionally induced insulin/insulin-like growth factor 1 (IGF-1) signalling (IIS) via phosphatidyl inositol-3-kinase (PI3K), phosphoinositide-dependent kinase 1 (PDK1 or PDPK1), and protein kinase B (Akt or PKB) in the follicular epithelium. We find similar results in the developing Drosophila wing, where Yki becomes nuclear in the mechanically stretched cells of the wing pouch during larval feeding, which induces IIS, but translocates to the cytoplasm upon cessation of feeding in the third instar stage. Inactivating Akt prevents nuclear Yki localisation in the wing disc, while ectopic activation of the insulin receptor, PI3K, or Akt/PKB is sufficient to maintain nuclear Yki in mechanically stimulated cells of the wing pouch even after feeding ceases. Finally, IIS also promotes YAP nuclear localisation in response to mechanical cues in mammalian skin epithelia. Thus, the Hippo pathway has a physiological function as an integrator of epithelial cell polarity, tissue mechanics, and nutritional cues to control cell proliferation and tissue growth in both Drosophila and mammals.
Citation: Borreguero-Muñoz N, Fletcher GC, Aguilar-Aragon M, Elbediwy A, Vincent-Mistiaen ZI, Thompson BJ (2019) The Hippo pathway integrates PI3K–Akt signals with mechanical and polarity cues to control tissue growth. PLoS Biol 17(10): e3000509. https://doi.org/10.1371/journal.pbio.3000509
Academic Editor: Kenneth Irvine, Rutgers The State University of New Jersey, UNITED STATES
Received: November 22, 2018; Accepted: October 3, 2019; Published: October 15, 2019
Copyright: © 2019 Borreguero-Muñoz et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: All relevant data are within the paper and its Supporting Information files.
Funding: This work was funded by the Francis Crick Institute core funding to BT (FC0011080). It was also funded by EMBL Australia & The John Curtin School of Medical Research at The Australian National University. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Abbreviations: 4E-BP, Elongation initiation factor 4E binding protein; AEL, after egg laying; ban.lacZ, bantam.lacZ; BIFC, bimolecular fluorescence complementation; Crb, Crumbs; Dcp1, Drosophila Death Caspase 1; Dilp, Drosophila insulin-like peptide; dp110caax, Drosophila p110-caax; DREF, DNA replication element binding factor; D–V, Dorsal–Ventral; EcR, ecdysone receptor; ex.lacZ, expanded.lacZ; Eya, Eyes Absent; FAK, Focal Adhesion Kinase; FOXO, Forkhead box O; GAP, GTPase-activating protein; GFP, green fluorescent protein; hh.Gal4, hedgehog.Gal4; Hpo, Hippo; IGF-1, insulin-like growth factor 1; IIS, insulin/IGF-1 signalling; Inr, insulin/IGF-1 receptor; IP, intraperitoneally; IR, Inverted Repeat Hairpin RNAi; LATS, Large tumour suppressor; LIMD1, LIM domain 1; MST, Mammalian Sterile 20 kinase; Myo-II, Myosin-II; NF2, Neurofibromatosis2; NLS, nuclear localisation signal; nlsRFP, nuclear red fluorescent protein; nub.Gal4, nubbin.Gal4; OvoD, Ovo dominant; PBST, PBS/0.1% Triton X-100; PBST/NGS, normal goat serum/PBST; PDK1, phosphoinositide-dependent protein kinase 1; PH, Pleckstrin Homology; PI3K, phosphatidyl inositol-3-kinase; PIK3CA, PI3K catalytic subunit alpha; PIP, phosphatidyl inositol phosphate; PKB, protein kinase B; Pol, RNA Polymerase; PRAS40, 40-kDa proline-rich Akt substrate; PTEN, phosphatase and tensin homolog; RFP, red fluorescent protein; Rheb, Ras-homolog enriched in the brain; RNAi, RNA interference; Rok, Rho-kinase; S6K, Ribosomal protein S6 kinase; Sd, Scalloped; Src, Rous Sarcoma Virus Oncogene; TAZ, Transcriptional Activator with a PDZ domain; TEAD, TEA domain; TIF, Transcription intermediary factor; tj.Gal4, trafficjam.Gal4; TOR, Target of Rapamycin; TORC1, TOR complex 1; TRIP6, Thyroid receptor interacting protein 6; TSC, Tuberous Sclerosis Complex; UAS, upstream activator sequence; UBF, Upstream Binding Factor; Wts, Warts; WWTR1, WW-domain–containing transcriptional coactivator; YAP, Yes-associated protein; Yki, Yorkie
The growth of animal tissues is known to depend on nutritionally induced circulating hormones of the insulin/insulin-like growth factor 1 (IGF-1) family [1–3]. In addition, tissue growth can be mechanically induced via the Hippo signalling pathway [4–8]. How these two mechanisms of tissue growth control are integrated during animal development remains unclear. The fruit fly Drosophila offers a tractable model system to explore how insulin/IGF-1 signalling (IIS) and the Hippo pathway interact to influence cell proliferation in multiple epithelial tissues during development. In Drosophila oogenesis, the developing oocyte in each egg chamber is fed cytoplasm by endoreplicating germline nurse cells that grow enormously in size by cell growth without cell division [9–13]. The somatic follicle cell epithelium that surrounds the germline grows by coordinated cell growth and cell division—cell proliferation—to precisely encapsulate each egg chamber during early stages of oogenesis (stages 1–7) . Proliferation of follicle cells is thought to occur in response to mechanical stretching caused by the growth of the underlying germline [15, 16]. Furthermore, growth of the entire egg chamber is known to depend on adequate nutrient intake by the adult female . After fertilisation of the egg, embryogenesis proceeds within the eggshell without the need for feeding or growth. At the end of embryogenesis, the hatching larvae is able to feed and grow via a similar subdivision of tissues into those growing without cell division (the endoreplicating larval tissues) and those growing by cell proliferation (the mitotic ‘imaginal discs’ that give rise to the future adult body or ‘imago’) [11, 12, 18]. The growth rate of the entire larva, including both endoreplicating and proliferating tissues, once again depends upon nutritional intake and thus contributes to the determination of adult body size [1, 2, 19].
The IIS pathway was found to be induced by nutritional cues in Drosophila [1–3, 20–23]. Nutrient intake stimulates production of circulating Drosophila insulin-like peptides (Dilps), which activate the insulin/IGF-1 receptor (InR), leading to the recruitment of the phosphatidyl inositol-3-kinase (PI3K—composed of two subunits, p60 and p110), which coverts phosphatidyl inositol phosphate (PIP)2 to PIP3 at the plasma membrane of signal-receiving cells (a process antagonised by the phosphatase and tensin homolog PTEN) [3, 20–30]. Induction of PIP3 leads to the recruitment of two Pleckstrin Homology (PH)-domain–containing kinases, phosphoinositide-dependent protein kinase 1 (PDK1) and Akt (also called protein kinase B [PKB]), enabling PDK1 to phosphorylate Akt, which is then responsible for signal transduction [31–37] and tissue growth control [38–41].
One important downstream effector of Akt is the Target of Rapamycin (TOR) complex 1 (TORC1), which promotes cell growth by inducing translation via Ribosomal protein S6 kinase (S6K) [39, 42, 43] and inactivating the translational inhibitor, Elongation initiating factor 4E binding protein (4E-BP) [43, 44]. TORC1 also induces ribosome biogenesis via the RNA Polymerase (Pol) II transcription factors Myc [45–49] and DNA replication element binding factor (DREF)  and the RNA Pol I activators Transcription intermediary factor 1A (TIF1A/Rrn3) [51, 52] and TIF1B/SL1-Upstream binding factor (UBF) , as well as by inactivating the RNA Pol III inhibitor Maf1 [54, 55]. TORC1 is composed of the TOR kinase, Raptor, and Lst8 subunits [56–59] and is activated by Ras-homolog enriched in the brain (Rheb) GTPase [60–62] at the lysosome [63, 64] and inhibited by the Tuberous Sclerosis Complex TSC1/2 GTPase-activating proteins (GAPs) [65–67] and the 40-kDa proline-rich Akt substrate (PRAS40) [68–70]. Akt appears to activate TORC1 by phosphorylating TSC2 to displace it from the lysosome [71, 72], although mutation of two Akt phosphorylation sites in TSC2 does not affect growth in Drosophila , suggesting that other Akt targets, such as PRAS40, may compensate. Importantly, a negative feedback loop operates in which TORC1 activation promotes cell growth but also functions to reduce phosphorylation and activation of Akt itself [74, 75].
Another target of Akt is the transcription factor Forkhead box O (FOXO), which, upon IIS activation, becomes phosphorylated by Akt to induce its retention in the cytoplasm [76–78]. Drosophila foxo mutants are viable and normally sized, but foxo is required for complete suppression of tissue growth upon reduced insulin/IGF-1–PI3K–Akt signalling, which sends FOXO to the nucleus to inhibit cell proliferation and promote apoptosis [79, 80]. Thus, Akt can act independently of the TORC1 complex to control cell proliferation rather than cell growth, raising the question of whether additional Akt substrates may exist that contribute to the control of tissue growth by the IIS pathway in proliferating tissues. The importance of this question is underscored by the fact that activation of PI3K–Akt signalling (in PI3K catalytic subunit alpha [PIK3CA] constitutively active mutant or in PTEN inactivating mutant tumours) is a widespread cause of malignant human cancer, while activation of TORC1 (in TSC1 or TSC2 mutant tumours) causes benign hamartomas [75, 81].
The Hippo signalling pathway was discovered by Drosophila genetics to restrict the rate of cell proliferation and final tissue size in developing wing and eye imaginal discs but does not affect cell growth in endoreplicating tissues [4–6]. The upstream kinase Hippo (Hpo) activates the downstream kinase Warts (Wts), which then directly inhibits the nuclear localisation of Yorkie (Yki), a transcriptional coactivator for Scalloped (Sd)/TEA domain (TEAD) DNA-binding proteins [82–84]. In mutants for hpo or wts, Yki translocates to the nucleus to switch Sd/TEAD from a repressor to an activator, which then drives cell proliferation and tissue growth in the developing wing and eye imaginal discs [83–86]. When mutant clones for yki are induced in the wing disc, cell proliferation is inhibited, and cells are eliminated by apoptosis [82, 87]. These dramatic phenotypes strongly suggest that the Hippo pathway might have a physiological role in tissue growth control in proliferating tissues, but it is still unclear how dynamic regulation of Yki nuclear localisation is controlled as tissues initiate or arrest their proliferation during development.
A physiological role for the Hippo pathway as a sensor of mechanical stress and strain in vivo was recently identified in Drosophila [88, 89]. Here, we explore how mechanical regulation of Hippo pathway integrates with nutritional control of tissue growth via the IIS pathway in the ovarian follicle cell epithelium and wing imaginal disc. Previous work indicated that genetic alteration of IIS can influence Hippo pathway signalling, but the physiological relevance of this observation and the molecular mechanisms responsible are still not fully understood . Here, we propose that insulin/IGF-1 act via Akt to inhibit Hippo pathway signalling and promote nuclear localisation of Yki in response to mechanical stress and strain. In the follicle cell epithelium, Yki responds primarily to mechanical strain driven by growth of the germline (itself insulin/IGF-1– and TORC1-dependent) but also requires PI3K–Akt signalling in follicle cells. In the wing imaginal disc, Yki responds to Fat–Dachsous signalling [4–8] and mechanical stress in columnar cells [89, 91–94], as well as to mechanical strain in flattened peripodial cells [88, 95], and we uncover an additional physiological regulation by nutritionally regulated IIS via PI3K–Akt. We further confirm a recent report that TORC1 is not required in the wing disc for nuclear localisation of Yki and that loss of TORC1 in fact drives Yki to the nucleus , which we attribute to feedback effects on PI3K–Akt. Finally, we confirm our findings in the mammalian skin epithelium, an example of a tissue in which both IIS and mechanically regulated Yes-associated protein (YAP) are crucial to promote cell proliferation.
We first examined early Drosophila oogenesis, where growth of the germline was shown to mechanically induce proliferation of surrounding follicle cells during stages 2–6 [15, 16]. We find that expression of the Yki reporter gene expanded.lacZ (ex.lacZ) is elevated and that green fluorescent protein (GFP)-tagged Yki localises to the nucleus in proliferating follicle cells of early-stage egg chambers (Fig 1A and 1B and S1 Fig). Since ex.lacZ suffers from perdurance of the lacZ-encoded beta-galactosidase protein, which can obscure effects over short timescales, we chose to focus on Yki–GFP localisation as a more dynamic readout. We noticed that Yki nuclear localisation exhibited some female-to-female variation, evident in the quantification of the nuclear/cytoplasmic ratio of wild-type females (Fig 1B). We wondered whether this variation might relate to the growth rate of the egg chambers. To test this notion, we arrested germline growth beyond stage 4 using Ovo dominant (OvoD) mutants, which we find prevents mechanical stretching of follicle cells and inhibits Yki nuclear localisation (Fig 1B). Note that in OvoD egg chambers, some nuclear Yki is still detectable prior to stage 4, but after stage 4, Yki is strongly cytoplasmic, as shown in the quantification (Fig 1B). Yki is known to promote follicle stem cell maintenance  and polar cell fate , but whether Yki is also involved in stretch-induced cell proliferation in follicle cells has not been explored. We find that Yki is essential for normal follicle cell proliferation because silencing of yki expression specifically in follicle cells by trafficjam.Gal4 (tj.Gal4)-driven transgenic Upstream activator sequence (UAS).yki-RNA interference (RNAi) reduces the number of phospho-Histone-H3–positive mitotic cells in each ovariole and profoundly disrupts oogenesis without affecting cell fate specification of follicle cells (marked by expression of Eyes Absent [Eya] and Broad) or follicle cell apoptosis (marked by Drosophila Death Caspase 1 [Dcp1] staining) (Fig 1C and 1D). Note that the insufficient number of follicle cells in the absence of Yki leads to germline apoptosis (Dcp1-positive)  (Fig 1D). Silencing of Sd by expression of UAS.sd-RNAi causes a milder phenotype, reducing follicle cell proliferation without disrupting germline growth during early stages (Fig 1C and 1D and S2 Fig). These results show that Yki subcellular localisation is dynamically patterned during early proliferative follicle cell development, becoming nuclear-localised in order for the Yki–Sd transcription factor to promote follicle cell proliferation during early egg chamber growth.
A) Expression of the Yki–Sd reporter gene ex.lacZ in early egg chambers is revealed by the pattern of nuclear beta-galactosidase immunostaining. Note that ex.lacZ is expressed during the stages in which mechanical stretch drives follicle cell proliferation. B) Expression and subcellular localisation of a Yki–GFP knockin line in early egg chambers reveals nuclear localisation of endogenous Yki during the stages of stretch-induced follicle cell proliferation. Quantification of the nuclear/cytoplasmic ratio of Yki–GFP is shown on the right (n > 30 per genotype; t test p < 0.05). See supplementary file S1_Data.xlsx for underlying data. C) Mitotic cells (pH3+) in the follicle cell epithelium are reduced upon expression of Yki–RNAi or Sd–RNAi. Numbers of follicle cells are reduced by both Yki–RNAi or Sd–RNAi, more weakly in the latter case. The Yki–RNAi phenotype is so strong that germ line cells are often affected by insufficiency in follicle cell numbers. Follicle cell fate, marked by expression of Eya, is not affected. The graph shows quantification of the average number of mitotic cells (pH3+) per egg chamber in each of the genotypes above (n > 10 egg chambers per genotype). For the Yki–RNA quantification, weaker phenotypes that still form individual egg chambers were used to measure pH3+ cells per egg chamber. See supplementary file S1_Data.xlsx for underlying data. D). Apoptosis, marked by Dcp1-positive cells, does not occur in follicle cell epithelia expressing Yki–RNAi or Sd–RNAi but does occur in germline cells affected by insufficiency in follicle cell numbers upon expression of Yki–RNAi. Follicle cell fate, marked by expression of Broad at stage 6 onward, is not affected by either Yki–RNAi or Sd–RNAi. Scale bars approximately 10 μM. Dcp1, Drosophila Death Caspase 1; ex.lacZ, expanded.lacZ; Eya, Eyes Absent; GFP, green fluorescent protein; IR, Inverted Repeat Hairpin RNAi; n/c, nuclear/cytoplasmic ratio; OvoD, Ovo dominant; pH3+, phospho-Histone-H3–positive; RNAi, RNA interference; Sd, Scalloped; WT, wild type; Yki, Yorkie.
The fact that the loss of Sd causes a weaker phenotype than loss of Yki is expected because Sd acts as default repressor such that loss of Yki prevents activation and leads to constitutive repression of Yki–Sd target genes, while loss of Sd prevents either activation or repression of target genes [86, 99]. Nevertheless, we sought to confirm that our UAS.sd-RNAi line was indeed causing a full loss of Sd function. Since Sd acts as a direct binding partner for Yki in the nucleus, it promotes Yki nuclear localisation [100–102]. We find that expression of UAS.sd-RNAi is sufficient to completely abolish Yki nuclear localisation in the follicle cell epithelium of both early- and late-stage egg chambers (S3A and S3B Fig). We therefore characterised the UAS.sd-RNAi phenotype in more detail and found that the resulting adult female animals are completely sterile because of arrest of egg chamber development at stage 10 of oogenesis (S3B Fig). When we examine such arrested stage 10 egg chambers, we observe that they lack sufficient follicle cells to cover the surface of the egg chamber, leading to subsequent apoptosis of germline cells (Dcp1-positive) (S3C Fig). These results show that strong Sd loss of function disrupts follicle cell proliferation such that there are insufficient cells to cover the germline and ensure its survival beyond stage 10 of oogenesis. This Sd loss-of-function phenotype confirms a physiological requirement for regulation of the Hippo pathway during follicle cell proliferation in vivo.
Since both follicle cell proliferation and germline growth are known to depend profoundly on nutritionally induced IIS [16, 17, 103, 104], we tested whether nutritional regulation of IIS in the germline cells might affect Yki subcellular localisation in the overlying follicle cell epithelium. We first compared the localisation of Yki–GFP in ovarioles from control (fed) adult females with those subjected to nutrient restriction for 24 h. We found that nutrient restriction caused a dramatic reduction in the nuclear localisation of Yki–GFP in follicle cells (Fig 2A). To test whether the effects of nutrient restriction were mediated by IIS to the germline, we induced null mutant clones of akt3 in the germline. We found that, as expected, cell growth is dramatically impaired in akt3 mutant germline cells and that this leads to relocalisation of Yki–GFP to the cytoplasm in the overlying follicle cell epithelium, which exhibits reduced cell proliferation (Fig 2B). The effect of Akt on germline growth is mediated by TORC1 because expression of UAS.TOR-RNAi in germline cells with the maternal tubulin.Gal4 driver reduces germline cell growth and is sufficient to reduce mechanical stretching and nuclear localisation of Yki–GFP in the surrounding follicle cell epithelium (S4 Fig). Thus, IIS acts on the germline to drive cell growth and thus indirectly induces mechanical stretching of the follicular epithelium and nuclear localisation of Yki in follicle cells.
A) Yki–GFP localises to the nucleus in early-stage ovarian follicle cells but relocalises to the cytoplasm upon nutrient restriction of adult females for 24 h. Quantification of the nuclear/cytoplasmic ratio is shown on the right (n > 30 per genotype, t test p < 0.05). Scale bars approximately 10 μM. See supplementary file S1_Data.xlsx for underlying data. B) Yki–GFP localises to the nucleus in early-stage ovarian follicle cells but relocalises to the cytoplasm upon induction of akt3 mutant clones in the germline, marked by the absence of nlsRFP. Note that follicle cells are wild type. Scale bars approximately 10 μM. C) Surface views of akt3 mutant germline clones from (B) allow quantification of n/c. Scale bars approximately 3 μM. See supplementary file S1_Data.xlsx for underlying data. GFP, green fluorescent protein; nlsRFP, nuclear red fluorescent protein; n/c, nuclear/cytoplasmic ratio; pH3, phospho-Histone H3; PI3K, phosphatidyl inositol-3-kinase; Yki, Yorkie.
We next tested whether IIS in the follicle cell epithelium itself affects Yki subcellular localisation because this pathway has previously been shown to act via PI3K and PDK1 to promote Yki activity in imaginal discs . We sought to examine the role of the key downstream effector of these kinases, Akt, whose potential role was previously overlooked because RNAi of Akt in S2 cells did not completely abolish the effect of insulin on Yki phosphorylation . We therefore induced mutant clones of akt3 in the follicle cell epithelium and found that Yki–GFP relocalises to the cytoplasm in these clones, even following strong cellular stretching at late stages of oogenesis (Fig 3A–3F).
A) Yki–GFP localisation to the nucleus is detectable in follicle cells at stage 4 of oogenesis. Scale bars approximately 10 μM. B) Yki–GFP localisation to the nucleus is weak or absent in follicle cells at stage 4 of oogenesis that are mutant for akt3. Note that germline cells are wild type. Scale bars approximately 10 μM. C) Yki–GFP localisation to the nucleus is weak or absent in follicle cells at stage 7 of oogenesis that are mutant for akt3. Scale bars approximately 10 μM. D) Yki–GFP localisation to the nucleus is weak or absent in follicle cells at stage 10 of oogenesis that are mutant for akt3. Scale bars approximately 10 μM. E) Yki–GFP localisation to the nucleus is weak or absent in follicle cells at stage 12 of oogenesis that are mutant for akt3. Scale bars approximately 10 μM. F) Yki–GFP localisation to the nucleus is weak or absent in follicle cells at stage 14 of oogenesis that are mutant for akt3. Scale bars approximately 10 μM. GFP, green fluorescent protein; nlsRFP, nuclear red fluorescent protein; Yki, Yorkie.
PI3K–PDK1–Akt signalling acts by regulating the canonical Hippo pathway because an Hpo dimerisation reporter, normally detectable only in columnar follicle cells and not in stretched cells , is strongly up-regulated upon inhibition of PI3K or Akt or overexpression of PTEN (Fig 4A–4C). The effect of Akt depends on canonical Hippo pathway signalling because double mutant akt3 wtsX1 clones still exhibit nuclear Yki–GFP localisation, even in columnar cells (Fig 4D). Furthermore, Yki nuclear localisation in highly stretched cells can be inhibited by treatment with two different PDK1 inhibitors, BX-795 and BX-912, whose effects are blocked by coexpression of UAS.Hpo-RNAi or UAS.Wts-RNAi (Fig 4E). The effect of Akt in follicle cells is not mediated by TORC1 because expression of dominant-negative UAS.TORTED or UAS.TOR-RNAi or induction of mutant clones for rheb does not prevent nuclear localisation of Yki–GFP (Fig 4F and 4G). Together, the above results show that IIS, via PI3K–PDK1–Akt, directly regulates the canonical Hippo pathway and is a prerequisite for nuclear localisation of Yki in both proliferating early-stage follicle cells and flattening late-stage stretch cells.
A) Expression of an Hpo KD BIFC sensor is detectable at the apical membrane of columnar follicle cells at stage 10 of oogenesis and is dramatically up-regulated upon coexpression of a dominant-negative PI3K p60 subunit (UAS.p60). A KA Hpo BIFC sensor is also dramatically up-regulated compared to the KD version. Scale bars approximately 10 μM. B) Expression of PTEN up-regulates the KD Hpo BIFC sensor in columnar follicle cells at stage 10 of oogenesis. Scale bars approximately 10 μM. C) Expression of Akt–RNAi up-regulates the KD Hpo BIFC sensor in columnar follicle cells at stage 10 of oogenesis. D) Yki–GFP localisation to the nucleus is weak or absent in follicle cells at stage 10 of oogenesis that are mutant for akt3 but is nuclear-localised in akt3 wtsX1 double mutant clones. Scale bars approximately 10 μM. E) Yki–GFP localises to the nucleus in stretch cells at stage 10 of oogenesis. Inhibiting PDK1 activity acutely with BX-795 or BX-912 blocks Yki–GFP nuclear localisation in a manner that depends on the canonical Hippo pathway kinases Hpo and Wts, whose knockdown with RNAi restores Yki–GFP nuclear localisation even in the presence of PDK1 inhibitors. F) Yki–GFP localises to the nucleus even upon inhibition of TORC1 by expression of dominant-negative TOR-TED or TOR-RNAi in stretch cells at stage 10 of oogenesis. G) Yki–GFP localises to the nucleus even upon inhibition of TORC1 by induction of rheb mutant clones at stage 14 of oogenesis. BIFC, bimolecular fluorescence complementation; DN, dominant-negative; GFP, green fluorescent protein; Hpo, Hippo; inh., inhibited; IR, Inverted Repeat Hairpain RNAi; KA, kinase-active; KD, kinase-dead; PDK1, phosphoinositide-dependent protein kinase 1; PI3K, phosphatidyl inositol-3-kinase; PTEN, phosphatase and tensin homolog; Rheb, Ras-homolog enriched in the brain; RNAi, RNA interference; tj.Gal4, trafficjam.Gal4; TOR, Target of Rapamycin; TORC1, TOR complex 1; UAS, Upstream activator sequence; Wts, Warts; Yki, Yorkie.
To confirm our findings in another Drosophila tissue, we examined the proliferating Drosophila larval wing imaginal disc, particularly the wing pouch, where the Hippo pathway has been shown to respond to gradients of Fat–Dachsous signalling [4–8] as well as physiological mechanical inputs, Ajuba–Wts-mediated stress sensing in the columnar cells of the wing pouch, and Hippo-pathway–mediated strain sensing in the overlying peripodial cells [89, 94] (S5–S7 Figs). Since experimental manipulation of IIS has been reported to influence Hippo pathway signalling via PI3K–PDK1 in the wing disc , we wondered whether physiological changes in IIS might affect Yki nuclear localisation during wing development. Towards the end of the third instar of larval development, feeding ceases, and larvae begin to wander out of the food as they prepare to form pupae and undergo metamorphosis. Wing disc cell proliferation slows and subsequently arrests at this point, with final size determined by a combination of reduced IIS from the brain and a surge of ecdysone signalling that triggers pupariation and metamorphosis [21, 23, 105]. We tested whether this physiological change in IIS might regulate Yki–GFP as the wing disc slows and arrests proliferation at the end of the third instar. We find that nuclear Yki–GFP localisation is prominent during early stages but is reduced by the late third instar stage when cessation of larval feeding occurs (Fig 5A and S7 Fig). Reducing Akt signalling by expression of akt–RNAi or subjecting early third instar larvae to nutrient restriction for 24 h was sufficient to reduce Yki–GFP nuclear localisation (Fig 5B). Furthermore, the pattern of Yki nuclear localisation in early third instar wing discs can be maintained in late third instar wing discs by expressing insulin receptor (UAS.InR) or constitutively active forms of PI3K (UAS.dp110caax) or Akt (UAS.Akt-myr) in the posterior compartment with the hedgehog.Gal4 (hh.Gal4) driver (Fig 5C). We confirm that hh.Gal4-driven manipulation of PI3K–Akt signalling and manipulation of Yki activity in wing discs generates similar tissue growth phenotypes in adult wings, illustrating the importance of cell proliferation control in larval imaginal discs for determination of final tissue size (Fig 5D). These results support the notion that the interplay of Fat–Dachsous signalling and mechanical cues with nutritionally induced IIS, acting via PI3K–PDK1–Akt, controls Yki nuclear translocation to promote tissue growth in the Drosophila wing.
A) Yki–GFP localises to the nucleus in early second and third instar larval wing imaginal discs in a pattern that closely resembles that of mechanical stress and strain (see also S7 Fig). Yki–GFP localises much less strongly to the nucleus in late ‘wandering’ third instar larval wing imaginal discs. Note the cytoplasmic localisation in the central region and weak nuclear localisation at the dorsal ventral boundary and at the periphery at late L3. Quantification is shown on right (n > 10 per time point). Scale bars approximately 5 μM. See supplementary file S1_Data.xlsx for underlying data. B) Silencing of akt expression by UAS.akt-RNAi hairpin transgene prevents nuclear Yki–GFP localisation in the L2 wing disc. Reducing Akt signalling by nutrient restriction for 24 h also prevents nuclear localisation of Yki–GFP at early L3. Quantification is shown on right (n > 10 per time point). Scale bars approximately 5 μM. See supplementary file S1_Data.xlsx for underlying data. C) Activating PI3K–Akt signalling by overexpression of insulin receptor (hh.Gal4 UAS.InR), a membrane-targeted version of the PI3K catalytic subunit (hh.Gal4 UAS.dp110caax), or membrane-targeted Akt (hh.Gal4 UAS.akt-myr) in the P compartment is sufficient to maintain the early pattern of Yki–GFP nuclear localisation in the posterior compartment of late third instar wing discs. Compare A and P compartments. Scale bars approximately 5 μM. D) Adult wings showing similar tissue overgrowth and undergrowth phenotypes in the posterior compartment when hh.Gal4 is used to silence expression of pten or hpo (which causes P-compartment overgrowth) as well as akt and yki (which causes P-compartment undergrowth). A, anterior; AEL, after egg laying; dp110caax, Drosophila p110-caax; GFP, green fluorescent protein; hh.Gal4, hedgehog.Gal4; Hpo, Hippo; IGF-1, insulin-like growth factor 1; InR, insulin/IGF-1 receptor; n/c, nuclear/cytoplasmic ratio; P, posterior; PI3K, phosphatidyl inositol-3-kinase; PTEN, phosphatase and tensin homolog; RNAi, RNA interference; UAS, upstream activator sequence; Yki, Yorkie.
A recent report suggested that IIS also acts via TOR to regulate Yki . Interestingly, inhibition of TOR caused a strong ectopic localisation of Yki to the nucleus, even in late third instar imaginal discs . We confirmed these findings with our Yki–GFP line, which strongly accumulates in the nucleus when dominant-negative UAS.TORTED is expressed in the posterior compartment of the wing disc (S8A Fig). The increase in nuclear Yki–GFP is due to disruption of the TORC1–Akt negative feedback loop  because the effects of UAS.TORTED are reversed by treatment with PDK1 inhibitors (S8B Fig). Thus, IIS promotes cell proliferation in the wing disc via PI3K–PDK1–Akt inhibition of the Hippo pathway and additionally promotes cell growth via TORC1, which also provides negative-feedback–limit Akt signalling. Accordingly, ectopic activation of IIS drives both cell growth and division, producing larger tissues with larger cells [3, 106], while ectopic activation of Yki produces larger tissues composed of increased numbers of normally sized cells .
We note that some differences exist between the spatiotemporal pattern of Yki–GFP localisation and the pattern of the Yki reporter genes ex.lacZ and bantam.lacZ (ban.lacZ) in the wing disc (Fig 6A). For example, the strong nuclear localisation of Yki–GFP at the Dorsal–Ventral (D–V) boundary is not reflected in either ex.lacZ or ban.lacZ expression, and both target genes are instead repressed at the D–V boundary (Fig 6A). Recent results explain this discrepancy because Notch signalling at the D–V boundary was found to potently repress the ability of activated Yki to transcriptionally induce target gene expression in the wing disc . Thus, the combination of Fat–Dachsous signalling and mechanical and nutritional inputs determines Yki nuclear localisation in the wing, while other signalling pathways, such as Notch, can modulate the transcriptional output of Yki–Sd on specific target genes. Nevertheless, the resulting pattern of ex.lacZ or ban.lacZ—low medially and high in a circumferential pattern at the periphery (Fig 6A)—matches the pattern of Fat–Dachsous signalling and mechanical stretching previously proposed to complement the action of compartment boundary organisers [108, 109] and thus level out the rate of cell proliferation across the wing pouch [110–114].
A) Wing imaginal discs at early, mid, and late L3 showing expression patterns for Sd–GFP, Yki–GFP and two Yki target genes: ban.lacZ and ex.lacZ. Note the correlation between Yki–GFP nuclear localisation and its target genes at early L3, at which both are elevated in a circumferential pattern. Note also that the pattern of lacZ (beta-galactosidase) staining is maintained into late-stage L3 because of the perdurance of beta-galactosidase protein. Finally, both ban.lacZ and ex.lacZ target genes are normally repressed at the D–V boundary by Notch signalling, which prevents nuclear Yki–GFP from inducing them in this territory of the wing. Thus, only the circumferential activation of Yki–GFP is normally functional in the wing pouch, consistent with its proposed role in wing growth. B) Late L3 wing imaginal disc peripodial epithelial cells are strongly stretched and retain nuclear Yki–GFP. Note that this nuclear Yki–GFP localisation still depends on the low levels of Akt signalling occurring at this stage because the localisation becomes cytoplasmic in akt3 mutant clones (marked by the absence of nlsRFP). ban.lacZ, bantam-lacZ; D–V, Dorsal–Ventral; ex.lacZ, expanded.lacZ; GFP, green fluorescent protein; nlsRFP, nuclear red fluorescent protein; Sd, Scalloped; Yki, Yorkie.
To examine the mechanism by which Akt regulates the Hippo pathway in Drosophila, we tested whether a conserved Akt consensus phosphorylation site first identified in the human Hpo kinase homolog Mammalian Sterile 20 kinase (MST)2 in vitro [115–118] is required for control of tissue growth in Drosophila. The Akt phosphorylation site (T132) is located two amino acids downstream of the catalytic aspartate in the Hpo (and in human MST1/2) kinase domains, suggesting that Akt phosphorylation of might directly inhibit Hpo kinase activity (S9A–S9D Fig). A pan-Akt substrate phosphospecific antibody recognises the monomeric form of the Hpo kinase but not the active dimer, suggesting that phosphorylation by Akt may prevent dimerisation of Hpo (S9B Fig). We therefore tested whether mutation of the T132 residue would cause ectopic activation of the Hpo kinase in vivo. Using a landing site system for controlled expression of transgenes, we compared the effect of expressing wild-type Hpo versus phosphomutant HpoT132A in follicle cells. We find that wild-type Hpo mildly reduces the number of follicle cells, while HpoT132A dramatically reduces follicle cell numbers, exposing many gaps in the coverage of the germline (S9E Fig). Accordingly, Yki–GFP nuclear localisation is strongly inhibited by HpoT132A expression, even in stretched cells (S9E Fig). In the wing, we find that phosphomutant HpoT132A dramatically inhibits tissue growth compared with wild-type Hpo expression (S9F, S9G and S10 Figs). These results suggest that this highly conserved Akt phosphorylation site in Hpo–MST1/2 kinases (S11 Fig) may be functional in vivo, although Akt may also employ other mechanisms to regulate Hippo pathway signalling to control cell proliferation and tissue growth.
Because the Hippo pathway appears to effectively integrate PI3K–Akt signalling with either mechanical stress sensing (via Rho-kinase [Rok]–Ajuba–Wts) in the columnar cells of the wing disc or mechanical strain sensing (via reduced Hpo kinase activation) in follicle cell epithelium [89, 94], we sought to confirm that the Rok–Ajuba–Wts mechanism is indeed dispensable in follicle cells. Accordingly, mutant clones for rok2 or ajubaΔII induced in the follicle cell epithelium (marked by absence of red fluorescent protein [RFP]) has no effect on nuclear localisation of Yki–GFP in mechanically stretched follicle cells (S12 Fig). These results confirm that the Rok–Ajuba pathway is not required for regulation of the Hippo pathway by mechanical strain, and thus, that the Hippo pathway uses distinct mechanisms to sense stress and strain in Drosophila. Nevertheless, an input from PI3K–Akt is essential for Yki activation in response to either stress or strain, regardless of the mechanisms involved.
In mammals, the skin epithelium is an example of a tissue in which both IIS via Akt [119–125] and mechanically regulated YAP and Transcriptional Activator with a PDZ domain (TAZ) [126–130] are known to promote keratinocyte cell proliferation, tissue regeneration after wounding, and tumour formation. Previous work identified a key role for PI3K and PDK1 in promoting nuclear localisation of YAP in skin keratinocytes  and other cell types . We now find that treatment with Akt inhibitor is sufficient to prevent YAP nuclear localisation in keratinocytes, even when plated at a low density to induce mechanical stimulation via integrin adhesions (Fig 7A). We further find that treatment of densely packed keratinocytes (with cytoplasmic YAP) with IGF-1 is sufficient to promote YAP nuclear localisation in all but the most crowded cells, similar to inhibition of the Hpo orthologs MST1/2 (Fig 7B). Thus, activation of PI3K–Akt has a similar effect on YAP as inhibition of Hippo pathway signalling in these cells. Finally, in mouse skin, activation of Akt by skin-specific deletion of PTEN is sufficient to promote YAP nuclear localisation and tumour-like tissue overgrowth, similar to that induced by skin-specific expression of nuclear-localised YAP5SA (Fig 7C). Together, these results indicate that IIS via Akt inhibits the canonical Hippo pathway to promote nuclear localisation of YAP and tissue growth in mammalian skin.
A) Human skin keratinocytes (HaCaT) cultured in sparse conditions to induce nuclear localisation of YAP were treated with either control (DMSO) or Akt inhibitor (MK2206) at 1 μM for 4 hours prior to fixation and immunostaining for YAP, which becomes cytoplasmic upon Akt inhibition. B) Human skin keratinocytes (HaCaT) cultured in dense conditions to induce cytoplasmic localisation of YAP were treated with control (DMSO), IGF-1, or MST1/2 kinase inhibitor (XMU-MP-1) for 4 hours prior to fixation and immunostaining for YAP, which becomes nuclear upon IGF-1 activation or MST1/2 inhibition. C) Mouse skin from wild-type, skin-specific conditionally induced PTEN knockout or skin-specific conditionally induced nuclear NLS–YAP–5SA–overexpressing animals were immunostained for YAP (brown). Note similar nuclear localisation of YAP and tumour-like tissue overgrowth in both PTEN knockout and NLS–YAP–5SA skin. IGF-1, insulin-like growth factor 1; inh., inhibited; MST, Mammalian Sterile 20 kinase; NLS, nuclear localisation signal; PI3K, phosphatidyl inositol-3-kinase; PTEN, phosphatase and tensin homolog; YAP, Yes-associated protein.
Our results show that the Hippo pathway has a physiological function in integrating hormonal IIS with mechanical inputs and polarity cues to control tissue growth in two different proliferating epithelia of Drosophila as well as in mammalian skin. Although manipulation of the Hippo pathway was previously shown to strongly affect cell proliferation and tissue growth [4–6], as well as to respond to the Fat–Dachsous planar polarity pathway [4–8], mechanical stress [89, 91–94], and mechanical strain [88, 95], it was previously unclear whether the Hippo pathway was also physiologically regulated by hormonal insulin/IGF-1 signals to control tissue growth during development. Our findings support the view that Yki/YAP normally relocalise to the nucleus to drive cell proliferation in epithelial cells subject to both mechanical stimuli and growth factor signalling via the PI3K–PDK1–Akt pathway. Below, we discuss how the Hippo pathway integrates these cues in different tissue types and different animal species. We then consider how evolutionary changes in the structure of the epidermis between Drosophila and mammals impact the mechanisms involved .
In the Drosophila ovarian follicle cell epithelium, our results suggest that growth of the germline stretches the surrounding follicle cells to induce nuclear localisation Yki, which activates Sd-mediated transcription to promote cell proliferation (Figs 1 and 2). Note that previous investigation with ex.lacZ failed to identify an effect of germline growth on follicle cell Yki activity, most likely because of perdurance of the lacZ gene product, beta-galactosidase . The primary mechanism of mechanotransduction in this tissue involves the canonical Hippo pathway, which is activated by Crumbs (Crb)-mediated clustering of apical Hpo kinase containing complexes to promote Hpo dimerisation and transactivation and inactivated by mechanical strain to decluster the same complexes . In addition, our results show that follicle cells must receive an insulin/IGF-1 signal that activates PI3K–PDK1–Akt to inhibit the Hpo kinase, possibly via direct phosphorylation on a conserved Akt phosphorylation motif or via other mechanisms that are still to be elucidated (Figs 3 and 4; S9–S11 Figs). In the absence of sufficient PI3K–PDK1–Akt signalling in follicle cells, the Hpo kinase becomes abnormally active, and Yki is retained in the cytoplasm even following mechanical strain (Fig 4). We note that PI3K–PDK1–Akt signalling directly affects Hpo kinase activity but that Hpo kinase activity itself promotes dimerisation because a kinase-active Hpo dimerisation sensor is much more strongly dimerised than the kinase-dead version . Thus, the dimerisation and transactivation mechanism of the Hpo kinase enables it to integrate both mechanical inputs and hormonal insulin/IGF-1 signals in follicle cells. We note that the Hippo pathway continuously senses mechanical strain in the follicle cell epithelium  but only controls cell proliferation during the early stages (1–7) of oogenesis (Figs 1–3), after which Notch receptor and ecdysone receptor (EcR) activation terminates proliferation by inducing a switch to endoreplication [132, 133].
During Drosophila wing disc growth, cessation of larval feeding in the late third instar stage reduces IIS and leads to decreased Yki nuclear localisation as cell proliferation first slows and then ultimately arrests upon ecdysone-induced metamorphosis (Fig 5A). Our findings confirm previous work linking IIS via PI3K and PDK1 with regulation of the Hippo pathway in the wing  and extend it by providing a molecular mechanism—Akt-mediated regulation of Hpo signalling—and demonstrating the physiological significance of this mechanism in tissue growth control (Figs 5A–5D, 6A and 6B). Our results confirm that nuclear localisation of Yki occurs in both mechanically stressed cells (domains with high Rok and Myosin-II [Myo-II] along the D–V boundary) and in mechanically strained cells (strongly flattened peripodial cells), as well as cells with high Fat–Dachsous signalling (at the periphery of the wing pouch) (Figs 5A–5C, 6A and 6B; S7 Fig). Stress sensing occurs via Rok and Myo-II, which are known to promote localisation of the Wts/Large tumour suppressor (LATS) inhibitor Ajuba/LIM domain 1 (LIMD1)/Thyroid receptor interacting protein 6 (TRIP6) to adherens junctions, which promotes Yki activity in the wing disc [89, 94, 134–136] (S7B Fig). Strain sensing in peripodial cells and also follicle cells occurs via a distinct mechanism involving dilution of apical Hippo pathway components [88, 137], and thus, follicle cells do not require Rok or Ajuba to activate Yki (S12 Fig). Note that the strong Ajuba-driven nuclear localisation of Yki along the D–V boundary of the wing disc does not actually lead to pro-proliferative target gene activation because of antagonism by Notch signalling . Thus, the Yki target gene bantam, which, along with Myc, mediates much of the effect on Yki on cell proliferation [87, 138, 139], is activated in a circumferential pattern at the periphery of the wing pouch and repressed medially during the early larval stages (Fig 6A)—in agreement with proposed models for mechanical stretch-induced proliferation in this tissue [110–114] and with gradients of Fat–Dachsous signalling [4–8]. Note also that Ajuba-mediated Yki activation was recently proposed to decline over time in the wing disc because of reduced mechanical stress and/or increased compression of cells , and our finding that increased PI3K–Akt signalling restores Yki nuclear localisation (Fig 5C and S7B Fig) suggests that integration of both mechanics and hormonal input is necessary to explain the temporal regulation of Yki.
The role of Myc as a downstream target of PI3K–Akt and Yki is particularly interesting because Myc not only stimulates cell proliferation and drives cell competition but also provides positive feedback on PI3K–Akt signalling itself . Thus, nutritional regulation of growth in Drosophila involves insulin/IGF-1–mediated signalling via PI3K–Akt, which can stabilise the Myc protein but also drive expression of the myc gene via activation of Yki–Sd (in the context of sufficient mechanical input) to sustain a feed-forward loop that drives further signalling and growth. Starvation-induced loss of IIS or insufficient mechanical input due to developmental defects might thus rapidly slow growth until nutrition is located or normally coordinated development is restored.
In mammalian skin, squamous epithelial cells lack a classical apical domain typical of columnar epithelia. Instead, basal layer cells contact the underlying extracellular matrix via basal integrin adhesions, which are important for stem cell proliferation [141–143] and to promote YAP/TAZ activation via multiple mechanisms, including activation of Focal Adhesion Kinase (FAK) and Rous Sarcoma Virus Oncogene (Src)-family kinase signalling [7, 8, 93, 126]. Src can directly phosphorylate YAP on three tyrosine residues to promote its activation  and was also reported to inhibit the LATS1 kinase in mammals . Integrin signalling can also activate PAK1 to inhibit membrane association of the key upstream Hippo pathway activator Merlin/Neurofibromatosis2 (NF2) [146–153]. Notably, integrins are generally dispensable for regulation of the Hippo pathway in Drosophila species, which have a columnar epidermis and can thus regulate Hippo pathway signalling via the apical domain as described above . Accordingly, Drosophila Yki lacks the tyrosine residues phosphorylated by Src in mammalian YAP, and Drosophila Merlin lacks the PAK1 phosphorylation site from mammalian Merlin/NF2.
Despite this divergence in mechanotransduction mechanisms between Drosophila and mammals, the Akt site in Hpo is conserved in MST1/2 [115–118], and our results indicate that integration of mechanical signalling and IIS is also a fundamentally conserved feature across metazoa. As in Drosophila, growth-factor–induced PI3K signalling is necessary for nuclear localisation of mammalian YAP [93, 126, 131], and our data show that this effect requires Akt activity and that IGF-1 is sufficient to promote nuclear localisation of YAP in response to mechanical stimulation in human keratinocytes (Fig 7). In mice, activation of PI3K–PDK1–Akt in conditional knockout PTENflox/flox skin  also promotes YAP nuclear localisation and skin proliferation, similar to conditionally induced expression of activated form of YAP (nlsYAP5SA) (Fig 7), confirming that YAP acts as an integrator of mechanical cues and IIS via PI3K–PDK1–Akt in skin cells both in culture and in vivo.
In conclusion, a key physiological function for the Hippo pathway is to integrate input from epithelial cell polarity determinants, mechanical cues, and hormonal IIS to promote cell proliferation and tissue growth in both Drosophila epithelia and mammalian skin. Although mechanisms of mechanotransduction via the Hippo pathway differ in the monolayered columnar epidermis of Drosophila versus the stratified squamous epidermis of mammals, growth factor signalling acts via a common PI3K–PDK1–Akt-mediated mechanism to inhibit the Hippo pathway and thus promote tissue growth. Thus, the Hippo signalling pathway could be considered as one of the key effectors of Akt in tissue growth control, alongside inhibition of FOXO and the classical inhibition of TSC1/2 to activate TORC1 (S13 Fig). Notably, our results show that activation of Akt alone is not sufficient to activate Yki because some type of mechanical stimulus is also necessary. In the absence of significant mechanical inputs, Akt acts primarily via TORC1 and FOXO, and the postmitotic Drosophila pupal retina appears to exemplify this mode of action—a phenomenon that helped distinguish and delineate PI3K–Akt and Hippo–Yki as separate pathways in pioneering genetic screens. Nevertheless, the widespread coupling of PI3K–Akt and Hippo pathway signalling in many tissues is potentially of major significance for human cancer because activation of PI3K–Akt signalling (in PIK3CA or PTEN mutant cells) causes formation of highly proliferative malignant tumours, while mutation of TSC1 or TSC2 leads to formation of relatively benign tumours [75, 81]. Given the increasing evidence for a potent role of YAP/TAZ in malignant tumours, future work should examine whether the Hippo pathway might be the primary effector of PI3K–Akt signalling in human cancer and thus a critical target for therapy.
Materials and methods
All animal-regulated procedures were carried out according to Project License constraints (PPL 70/7926) and United Kingdom Home Office guidelines and regulations. All experiments were carried out in accordance with the UK Animal Scientific Procedures Act (1986). The Francis Crick Institute Animal Ethics committee was the responsible party for approving animal care and use under this project licence. The research did not involve human participants.
Expression of UAS-driven transgenes in ovarian follicle cells was performed with the TJ.Gal4 driver and in wing imaginal disc cells with the hh.Gal4 driver, which is expressed in the posterior compartment, or the nubbin.Gal4 (nub.Gal4) driver, which is expressed in the entire wing pouch. Depletion of Yki in the follicle cell epithelium was driven by a strong UAS.Yki-RNAi (BL34067) using the TJ.Gal4 driver. Depletion of Sd in the follicle cell epithelium was driven by a strong UAS.Sd-RNAi (VDRC KK101497) using the TJ.Gal4 driver. Fly crosses were kept at a temperature of 25 °C. Ovaries were dissected and immunostained from adult females 4 days after eclosion. Larvae were dissected at stage L3 of development. After dissection, samples were fixed in 4% paraformaldehyde and processed for imaging.
CRISPR/Cas9 genome editing was used to tag the C-terminus of Yki with eGFP. 100 ng/μl of guide RNA plasmid (pCFD3, Addgene 49410, encoding the gRNA 5′-TCAGGTTTGTGGGAAGACGG-3′; Addgene, Cambridge, MA, USA), plus 500 ng/μl of a homologous recombination repair template plasmid, were coinjected into nos-Cas9 embryos. The repair template contained 4.5 kb genomic DNA from the Yki locus (centred around the stop codon), with eGFP inserted in-frame after the final amino acid of Yki and before its stop codon. The gRNA target sequence in the repair template was mutagenised to prevent recutting of correctly targeted alleles. The resulting knockin allele is homozygous viable .
The Drosophila genotypes used were as follows:
Ovaries and imaginal discs were dissected in PBS, fixed for 20 mins in 4% paraformaldehyde in PBS, washed for 30 minutes in PBS/0.1% Triton X-100 (PBST), and blocked for 15 minutes in 5% normal goat serum/PBST (PBST/NGS). Primary antibodies were diluted in PBST/NGS, and samples were incubated overnight at 4 °C.
The primary antibodies used were mouse anti-βgal (1:500; Promega, Madison, WI, USA), FITC-conjugated anti-GFP (1:400; Abcam, Cambridge, UK), mouse anti-Eya (1:250, DSHB), and mouse anti-Armadillo (1:100, Developmental Studies Hybrid Bank [DSHB], University of Iowa, Iowa City, IA, USA).
Secondary antibodies (all from Molecular Probes, Invitrogen, Carlsbad, CA, USA) were used at 1:500 for 2–4 hours prior to multiple washes in PBST and staining with DAPI at 1 μg/ml for 10–30 min prior to mounting on slides in Vectashield (Vector Laboratories, Burlingame, CA, USA).
Drosophila image acquisition
Confocal images were taken with a Leica SP5 confocal microscope (Wetzlar, Germany) using 20× and 40× oil immersion objectives and processed with Adobe Photoshop and Fiji. Either optical cross-sections through the middle of the different tissues or the top focal plane are shown in all figures. Pictures of the adult wings mounted in Hoyer’s medium were taken on a Zeiss Axioplan 2 Imaging Microscope (Oberkochen, Germany).
Human HaCAT cells (Francis Crick Institute cell services) were grown in DMEM (Gibco 41966; Gaithersburg, MD, USA) with 10% FCS and penicillin/streptomycin. All cells are subject to mycoplasma testing. Cells were treated with the Akt inhibitor MK2206 or the MST1/2 inhibitor XMU-MP-1 for 4 hours before being fixed with 4% PFA for 15 minutes before immunostaining.
Cell culture antibodies, image acquisition, and quantification
The primary antibodies used were mouse YAP (Santa Cruz sc-101199) 1:100. Secondary antibodies were from Invitrogen and used at 1:500 for 2 hours at room temperature along with DAPI. Cell culture samples were imaged with a Leica SP5 confocal microscope using a 63× oil immersion objective and processed using Adobe Photoshop. Cells were assessed over three independent experiments, counting 200–300 cells per condition.
Conditional activation of Cre recombinase in adult epidermis. Tamoxifen (20 mg/ml in con oil; Sigma-Aldrich, St. Louis, MO, USA) was injected intraperitoneally (IP) (5 μl/g body weight) for 5 consecutive days into 8- to 16-week–old control animals or transgenic animals carrying K5–CreERt Yap R26–YAP5SA–NLS to induce YAP5SA–NLS expression and analysed for LacZ (lineage tracer) expression by immunohistochemistry from 3 days thereafter . Similar experiments were performed for the PTEN flox/flox conditional knockout skin, as described in .
Mouse skin samples were harvested and fixed in neutral-buffered formaldehyde 10% vol/vol (Sigma-Aldrich) and then embedded in paraffin in a head-to-tail orientation. The tissues were processed, embedded, and sectioned at 4 μm and used for haematoxylin–eosin staining and immunohistochemistry. Sections were dewaxed in xylene and dehydrated by passage through graded alcohols to water. If required for antigen retrieval, sections were microwaved in citrate buffer (pH 6) for 15 minutes and then transferred to PBS. Endogenous peroxidase was blocked using 1.6% hydrogen peroxide in PBS for 10 minutes, followed by washing in distilled water. Species-specific blocking serum (diluted to 10% in 1% BSA) was used to block nonspecific staining in the tissue for 30 minutes. Slides were incubated with primary antibody diluted to 1:100 in 1% BSA for 1 hour at room temperature. Sections were washed in PBS prior to applying the appropriate biotinylated secondary antibody for 45 min at room temperature. Sections were then washed in PBS and then incubated in ABC (Vector Laboratories PK-6100) for 30 minutes. Following washing in PBS, DAB solution was applied for 2–5 minutes with development of the colour reaction being monitored microscopically. Slides were washed in tap water, stained with a light haematoxylin, dehydrated, cleared, and then mounted. Antibodies used for IHC were YAP Cell signalling (14074) 1/400 O/N. Images were acquired with a Zeiss light microscope using 40× and 20× objectives.
S1 Fig. Yki–Venus localises to the nucleus in the mechanically stretched cells of the follicle cell epithelium during Drosophila oogenesis.
A) A Yki–Venus knockin line behaves identically to the Yki–GFP line. Note nuclear localisation in follicle cells at early stages of oogenesis. DAPI (blue) marks nuclei. B) At stage 10 of oogenesis, the Yki–Venus knockin line again behaves identically to the Yki–GFP line, showing nuclear localisation in stretch cells (anterior, left) but not columnar cells that contact the oocyte (posterior, right). GFP, green fluorescent protein; Yki, Yorkie.
S2 Fig. Sd localises constitutively to the nucleus in the follicle cell epithelium throughout Drosophila oogenesis.
A) An Sd–GFP knockin line localises to the nucleus in all follicle cells at early stages of oogenesis. F-actin is costained in red. B) An Sd–GFP knockin line localises to the nucleus in all follicle cells at stages 6–10 of oogenesis. F-actin is costained in red. DAPI marks nuclei in blue. C) An Sd–GFP knockin line localises to the nucleus in all follicle cells at stage 14 of oogenesis. DAPI marks nuclei in blue. GFP, green fluorescent protein; Sd, Scalloped.
S3 Fig. Loss of Sd prevents Yki nuclear localisation and causes arrest of egg chamber development at stage 10.
A) Expression of Sd–RNAi prevents nuclear localisation of Yki–GFP in early-stage egg chambers. Compare with Fig 1B. B) Expression of Sd–RNAi prevents nuclear localisation of Yki–GFP in late-stage egg chambers, including stretch cells at stage 10. C) Apoptosis, marked by Dcp1-positive cells, occurs in stage 10 germline cells affected by insufficiency in follicle cell numbers upon expression of Sd–RNAi. The Sd loss-of-function phenotype is a weaker version of the Yki loss-of-function phenotype; compare with Fig 1D. Dcp1, Drosophila Death Caspase 1; GFP, green fluorescent protein; RNAi, RNA interference; Sd, Scalloped; Yki, Yorkie.
S4 Fig. Tor-driven germline cell growth is required for flattening of ‘stretch cells’ at stage 9 of oogenesis at which Yki becomes strongly nuclear.
A) Yki–GFP localises to the nucleus in stretch cells and to the cytoplasm in columnar cells of the follicular epithelium at stage 9 of oogenesis. DAPI marks nuclei in blue. F-actin is costained in red. B) Yki–GFP localises to the cytoplasm in all cells when germline growth is arrested by silencing of Tor by expression of UAS.tor-RNAi specifically in germline cells with the maternal tub.Gal4 driver line. Note failure of stretch cells to become flattened in this stage 9 egg chamber. C) Yki–GFP localises to the cytoplasm in all cells when germline growth is arrested by silencing of Tor by expression of UAS.tor-RNAi specifically in germline cells with the maternal tub.Gal4 driver line. Note failure of stretch cells to become flattened in this stage 8 egg chamber. GFP, green fluorescent protein; RNAi, RNA interference; TOR, Target of Rapamycin; tub.Gal4, tubulin.Gal4; UAS, Upstream activator sequence; Yki, Yorkie.
S5 Fig. Sd–GFP expression pattern in imaginal discs.
A) Yki–GFP expression is shown in the wing disc proper, the wing disc peripodial epithelium, the eye disc, the eye disc peripodial epithelium, the leg disc, and the haltere disc. GFP, green fluorescent protein; Sd, Scalloped; Yki, Yorkie.
S6 Fig. Yki–GFP expression pattern in eye and leg imaginal discs.
A) Eye imaginal discs at early, mid, and late third instar (L3) stages, showing frequent nuclear Yki–GFP in early stages and predominantly cytoplasmic Yki–GFP at late stages. Note the strong nuclear Yki–GFP in the flattened cells of the peripodial epithelium at the periphery. B) Leg imaginal discs at early, mid, and late third instar (L3) stages, showing frequent nuclear Yki–GFP in early stages and predominantly cytoplasmic Yki–GFP at late stages. Note the strong nuclear Yki–GFP in the flattened cells of the peripodial epithelium at the periphery. GFP, green fluorescent protein; Yki, Yorkie.
S7 Fig. Yki–GFP nuclear localisation reflects apical domain stretching (strain) as well as the pattern of Rok-–GFP/Myo-II–GFP/Jub accumulation (stress) at the apical domain in the wing pouch.
A) Early, mid, and late third larval instar (L3) wing imaginal discs stained for Yki-–GFP knockin, endogenously expressed Myo-II/Sqh–GFP, and Rok–GFP expressed with nub.Gal4-driven UAS.Rok–GFP. Note correlation between Yki–GFP nuclear localisation and the pattern of mechanical stress and strain indicated by Myo-II/Sqh–GFP or Rok–GFP. B) Late-stage third larval instar (L3) wing imaginal disc immunostained for Jub and phospho-Src, both of which accumulate a junction in response to mechanical stress but not strain. GFP, green fluorescent protein; Jub, Ajuba; Myo-II, Myosin-II; nub.Gal4, nubbin.Gal4; Rok, Rho-kinase; Sqh, Spaghetti Squash; Src, Rous Sarcoma Virus Oncogene; Yki, Yorkie.
S8 Fig. Expression of a dominant-negative form of tor (torTED) in the posterior compartment of the wing disc increases Yki nuclear translocation via feedback effects on PDK1–Akt activity.
A) Upon inhibition of TOR activity by expression of hh.Gal4 UAS.torTED, there is an increase in Yki nuclear translocation in a group of cells. B) The UAS.torTED-driven nuclear translocation of Yki is inhibited by the PDK1 kinase inhibitor BX-795, indicating that TOR activity normally drives a negative feedback loop to inhibit PI3K–PDK1–Akt signalling, disruption of which leads to PDK1–Akt hyperactivation and Yki nuclear translocation in the wing. hh.Gal4, hedgehog.Gal4; PDK1, phosphoinositide-dependent kinase 1; PI3K, phosphatidyl inositol-3-kinase; TOR, Target of Rapamycin; UAS, Upstream activator sequence; Yki, Yorkie.
S9 Fig. An Akt phosphorylation site (T132) modulates Hpo kinase activity in vivo.
A) Sequence of the Hpo kinase domain showing location of the catalytic aspartate residue adjacent to the Akt phosphorylation site. B) Conservation of the Akt phosphorylation site motif between Drosophila Hpo and human MST1/2, but not in the non-Hippo pathway kinases MST3/4. A pan-Akt substrate phosphospecific antibody recognises monomeric immunoprecipitated Hpo kinase but not the dimeric form, suggesting that Akt phosphorylation may inhibit Hpo dimerisation in S2 cells. C) Diagram of the Hpo kinase structure showing the surface accessibility of the Akt phosphorylation site adjacent to the ATP binding cleft. D) Close-up of the loop connecting the Akt phosphorylation site with the catalytic aspartate residue. E) Expression of wild-type Hpo from a third chromosome landing site causes a mild reduction in the number of follicle cells, with occasional gaps in the epithelium(*). Expression of phosphomutant HpoT132A from the same landing site causes a strong reduction in the number of follicle cells, with frequent gaps in the epithelium(*) and a failure of posterior cells to columnarise (arrow). Yki–GFP remains cytoplasmic, even in highly stretched cells, upon expression of HpoT132A. F) Expression of wild-type Hpo from a third chromosome landing site causes a mild reduction in wing size, while expression of phosphomutant HpoT132 from the same landing site causes a dramatic reduction in wing size. G) Quantification of F. See supplementary file S1_Data.xlsx for underlying data. GFP, green fluorescent protein; Hpo, Hippo; MST, Mammalian Sterile 20 kinase; Yki, Yorkie.
S10 Fig. Genetic epistasis between overexpressed active Akt and overexpressed Hpo kinases.
A) Wing-specific nub.Gal4-driven expression of UAS.myr–Akt induces wing overgrowth. Overexpression of strongly active UAS.hpoT132A prevents wing growth and also prevents coexpressed UAS.myr–Akt from driving growth. B) Quantification of wing area from A. See supplementary file S1_Data.xlsx for underlying data. Hpo, Hippo; nub.Gal4, nubbin.Gal4; UAS, Upstream activator sequence.
S11 Fig. Conservation of the Akt site in MST1/2 and Hpo across metazoa.
Alignment of the Akt phosphorylation consensus motif in MST1/2 but not MST3/4 orthologs across metazoans. Hpo, Hippo; MST, Mammalian Sterile 20 kinase.
S12 Fig. The Rok/Jub mechanical stress sensing pathway is not required for Yki–GFP nuclear localisation in stretched follicle cells.
A) No effect on nuclear Yki–GFP localisation in Rok mutant (rok2) clones, marked by absence of nlsRFP in mechanically stretched follicle cells. B) No effect on nuclear Yki–GFP localisation in Jub mutant (jubΔ2) clones, marked by absence of nlsRFP in mechanically stretched follicle cells. Inset shows surface views of early stage 4 egg chamber. GFP, green fluorescent protein; Jub, Ajuba; nlsRFP, nuclear red fluorescent protein; Rok, Rho-kinase; Yki, Yorkie.
S13 Fig. Schematic diagram of Hippo signalling integrating PI3K-–Akt, mechanical, and polarity cues.
- 1. Edgar BA. How flies get their size: genetics meets physiology. Nat Rev Genet. 2006;7(12):907–16. pmid:17139322.
- 2. Hietakangas V, Cohen SM. Regulation of tissue growth through nutrient sensing. Annu Rev Genet. 2009;43:389–410. pmid:19694515.
- 3. Oldham S, Hafen E. Insulin/IGF and target of rapamycin signaling: a TOR de force in growth control. Trends Cell Biol. 2003;13(2):79–85. pmid:12559758.
- 4. Pan D. The hippo signaling pathway in development and cancer. Dev Cell. 2010;19(4):491–505. pmid:20951342
- 5. Harvey KF, Hariharan IK. The hippo pathway. Cold Spring Harb Perspect Biol. 2012;4(8):a011288. pmid:22745287
- 6. Halder G, Johnson RL. Hippo signaling: growth control and beyond. Development. 2011;138(1):9–22. pmid:21138973
- 7. Elbediwy A, Vincent-Mistiaen ZI, Thompson BJ. YAP and TAZ in epithelial stem cells: A sensor for cell polarity, mechanical forces and tissue damage. Bioessays. 2016;38(7):644–53. pmid:27173018.
- 8. Elbediwy A, Thompson BJ. Evolution of mechanotransduction via YAP/TAZ in animal epithelia. Curr Opin Cell Biol. 2018;51:117–23. pmid:29477107.
- 9. Spradling AC. Germline cysts: communes that work. Cell. 1993;72(5):649–51. pmid:8453660.
- 10. Bastock R, St Johnston D. Drosophila oogenesis. Curr Biol. 2008;18(23):R1082–7. pmid:19081037.
- 11. Edgar BA, Orr-Weaver TL. Endoreplication cell cycles: more for less. Cell. 2001;105(3):297–306. pmid:11348589.
- 12. Saucedo LJ, Edgar BA. Why size matters: altering cell size. Curr Opin Genet Dev. 2002;12(5):565–71. pmid:12200162.
- 13. Edgar BA, Zielke N, Gutierrez C. Endocycles: a recurrent evolutionary innovation for post-mitotic cell growth. Nat Rev Mol Cell Biol. 2014;15(3):197–210. pmid:24556841.
- 14. Horne-Badovinac S, Bilder D. Mass transit: epithelial morphogenesis in the Drosophila egg chamber. Dev Dyn. 2005;232(3):559–74. pmid:15704134.
- 15. Wang Y, Riechmann V. The role of the actomyosin cytoskeleton in coordination of tissue growth during Drosophila oogenesis. Curr Biol. 2007;17(15):1349–55. pmid:17656094.
- 16. Vachias C, Fritsch C, Pouchin P, Bardot O, Mirouse V. Tight coordination of growth and differentiation between germline and soma provides robustness for drosophila egg development. Cell Rep. 2014;9(2):531–41. pmid:25373901.
- 17. Drummond-Barbosa D, Spradling AC. Stem cells and their progeny respond to nutritional changes during Drosophila oogenesis. Dev Biol. 2001;231(1):265–78. pmid:11180967.
- 18. Thompson BJ. Developmental control of cell growth and division in Drosophila. Curr Opin Cell Biol. 2010;22(6):788–94. pmid:20833011.
- 19. Britton JS, Edgar BA. Environmental control of the cell cycle in Drosophila: nutrition activates mitotic and endoreplicative cells by distinct mechanisms. Development. 1998;125(11):2149–58. pmid:9570778.
- 20. Brogiolo W, Stocker H, Ikeya T, Rintelen F, Fernandez R, Hafen E. An evolutionarily conserved function of the Drosophila insulin receptor and insulin-like peptides in growth control. Curr Biol. 2001;11(4):213–21. pmid:11250149.
- 21. Ikeya T, Galic M, Belawat P, Nairz K, Hafen E. Nutrient-dependent expression of insulin-like peptides from neuroendocrine cells in the CNS contributes to growth regulation in Drosophila. Curr Biol. 2002;12(15):1293–300. pmid:12176357.
- 22. Britton JS, Lockwood WK, Li L, Cohen SM, Edgar BA. Drosophila’s insulin/PI3-kinase pathway coordinates cellular metabolism with nutritional conditions. Dev Cell. 2002;2(2):239–49. pmid:11832249.
- 23. Rulifson EJ, Kim SK, Nusse R. Ablation of insulin-producing neurons in flies: growth and diabetic phenotypes. Science. 2002;296(5570):1118–20. pmid:12004130.
- 24. Ruderman NB, Kapeller R, White MF, Cantley LC. Activation of phosphatidylinositol 3-kinase by insulin. Proc Natl Acad Sci U S A. 1990;87(4):1411–5. pmid:2154747
- 25. Carpenter CL, Duckworth BC, Auger KR, Cohen B, Schaffhausen BS, Cantley LC. Purification and characterization of phosphoinositide 3-kinase from rat liver. J Biol Chem. 1990;265(32):19704–11. pmid:2174051.
- 26. Kapeller R, Chen KS, Yoakim M, Schaffhausen BS, Backer J, White MF, et al. Mutations in the juxtamembrane region of the insulin receptor impair activation of phosphatidylinositol 3-kinase by insulin. Mol Endocrinol. 1991;5(6):769–77. pmid:1656240.
- 27. Leevers SJ, Weinkove D, MacDougall LK, Hafen E, Waterfield MD. The Drosophila phosphoinositide 3-kinase Dp110 promotes cell growth. EMBO J. 1996;15(23):6584–94. pmid:8978685
- 28. Weinkove D, Neufeld TP, Twardzik T, Waterfield MD, Leevers SJ. Regulation of imaginal disc cell size, cell number and organ size by Drosophila class I(A) phosphoinositide 3-kinase and its adaptor. Curr Biol. 1999;9(18):1019–29. pmid:10508611.
- 29. Bohni R, Riesgo-Escovar J, Oldham S, Brogiolo W, Stocker H, Andruss BF, et al. Autonomous control of cell and organ size by CHICO, a Drosophila homolog of vertebrate IRS1-4. Cell. 1999;97(7):865–75. pmid:10399915.
- 30. Oldham S, Stocker H, Laffargue M, Wittwer F, Wymann M, Hafen E. The Drosophila insulin/IGF receptor controls growth and size by modulating PtdInsP(3) levels. Development. 2002;129(17):4103–9. pmid:12163412.
- 31. Bellacosa A, Testa JR, Staal SP, Tsichlis PN. A retroviral oncogene, akt, encoding a serine-threonine kinase containing an SH2-like region. Science. 1991;254(5029):274–7. pmid:1833819.
- 32. Cross DA, Alessi DR, Cohen P, Andjelkovich M, Hemmings BA. Inhibition of glycogen synthase kinase-3 by insulin mediated by protein kinase B. Nature. 1995;378(6559):785–9. pmid:8524413.
- 33. Alessi DR, Andjelkovic M, Caudwell B, Cron P, Morrice N, Cohen P, et al. Mechanism of activation of protein kinase B by insulin and IGF-1. EMBO J. 1996;15(23):6541–51. pmid:8978681
- 34. Burgering BM, Coffer PJ. Protein kinase B (c-Akt) in phosphatidylinositol-3-OH kinase signal transduction. Nature. 1995;376(6541):599–602. pmid:7637810.
- 35. Franke TF, Yang SI, Chan TO, Datta K, Kazlauskas A, Morrison DK, et al. The protein kinase encoded by the Akt proto-oncogene is a target of the PDGF-activated phosphatidylinositol 3-kinase. Cell. 1995;81(5):727–36. pmid:7774014.
- 36. Franke TF, Kaplan DR, Cantley LC, Toker A. Direct regulation of the Akt proto-oncogene product by phosphatidylinositol-3,4-bisphosphate. Science. 1997;275(5300):665–8. pmid:9005852.
- 37. Franke TF, Kaplan DR, Cantley LC. PI3K: downstream AKTion blocks apoptosis. Cell. 1997;88(4):435–7. pmid:9038334.
- 38. Staveley BE, Ruel L, Jin J, Stambolic V, Mastronardi FG, Heitzler P, et al. Genetic analysis of protein kinase B (AKT) in Drosophila. Curr Biol. 1998;8(10):599–602. pmid:9601646.
- 39. Rintelen F, Stocker H, Thomas G, Hafen E. PDK1 regulates growth through Akt and S6K in Drosophila. Proc Natl Acad Sci U S A. 2001;98(26):15020–5. pmid:11752451
- 40. Verdu J, Buratovich MA, Wilder EL, Birnbaum MJ. Cell-autonomous regulation of cell and organ growth in Drosophila by Akt/PKB. Nat Cell Biol. 1999;1(8):500–6. pmid:10587646.
- 41. Stocker H, Andjelkovic M, Oldham S, Laffargue M, Wymann MP, Hemmings BA, et al. Living with lethal PIP3 levels: viability of flies lacking PTEN restored by a PH domain mutation in Akt/PKB. Science. 2002;295(5562):2088–91. pmid:11872800.
- 42. Zhang H, Stallock JP, Ng JC, Reinhard C, Neufeld TP. Regulation of cellular growth by the Drosophila target of rapamycin dTOR. Genes Dev. 2000;14(21):2712–24. pmid:11069888
- 43. Miron M, Lasko P, Sonenberg N. Signaling from Akt to FRAP/TOR targets both 4E-BP and S6K in Drosophila melanogaster. Mol Cell Biol. 2003;23(24):9117–26. pmid:14645523
- 44. Miron M, Verdu J, Lachance PE, Birnbaum MJ, Lasko PF, Sonenberg N. The translational inhibitor 4E-BP is an effector of PI(3)K/Akt signalling and cell growth in Drosophila. Nat Cell Biol. 2001;3(6):596–601. pmid:11389445.
- 45. Pierce SB, Yost C, Britton JS, Loo LW, Flynn EM, Edgar BA, et al. dMyc is required for larval growth and endoreplication in Drosophila. Development. 2004;131(10):2317–27. pmid:15128666.
- 46. West MJ, Stoneley M, Willis AE. Translational induction of the c-myc oncogene via activation of the FRAP/TOR signalling pathway. Oncogene. 1998;17(6):769–80. pmid:9715279.
- 47. Teleman AA, Hietakangas V, Sayadian AC, Cohen SM. Nutritional control of protein biosynthetic capacity by insulin via Myc in Drosophila. Cell Metab. 2008;7(1):21–32. pmid:18177722.
- 48. Chan JC, Hannan KM, Riddell K, Ng PY, Peck A, Lee RS, et al. AKT promotes rRNA synthesis and cooperates with c-MYC to stimulate ribosome biogenesis in cancer. Sci Signal. 2011;4(188):ra56. pmid:21878679.
- 49. Mitchell NC, Tchoubrieva EB, Chahal A, Woods S, Lee A, Lin JI, et al. S6 Kinase is essential for MYC-dependent rDNA transcription in Drosophila. Cell Signal. 2015;27(10):2045–53. pmid:26215099.
- 50. Killip LE, Grewal SS. DREF is required for cell and organismal growth in Drosophila and functions downstream of the nutrition/TOR pathway. Dev Biol. 2012;371(2):191–202. pmid:22960233.
- 51. Mayer C, Zhao J, Yuan X, Grummt I. mTOR-dependent activation of the transcription factor TIF-IA links rRNA synthesis to nutrient availability. Genes Dev. 2004;18(4):423–34. pmid:15004009
- 52. Grewal SS, Evans JR, Edgar BA. Drosophila TIF-IA is required for ribosome synthesis and cell growth and is regulated by the TOR pathway. J Cell Biol. 2007;179(6):1105–13. pmid:18086911
- 53. Hannan KM, Brandenburger Y, Jenkins A, Sharkey K, Cavanaugh A, Rothblum L, et al. mTOR-dependent regulation of ribosomal gene transcription requires S6K1 and is mediated by phosphorylation of the carboxy-terminal activation domain of the nucleolar transcription factor UBF. Mol Cell Biol. 2003;23(23):8862–77. pmid:14612424
- 54. Marshall L, Rideout EJ, Grewal SS. Nutrient/TOR-dependent regulation of RNA polymerase III controls tissue and organismal growth in Drosophila. EMBO J. 2012;31(8):1916–30. pmid:22367393
- 55. Rideout EJ, Marshall L, Grewal SS. Drosophila RNA polymerase III repressor Maf1 controls body size and developmental timing by modulating tRNAiMet synthesis and systemic insulin signaling. Proc Natl Acad Sci U S A. 2012;109(4):1139–44. pmid:22228302
- 56. Barbet NC, Schneider U, Helliwell SB, Stansfield I, Tuite MF, Hall MN. TOR controls translation initiation and early G1 progression in yeast. Mol Biol Cell. 1996;7(1):25–42. pmid:8741837
- 57. Kim DH, Sarbassov DD, Ali SM, King JE, Latek RR, Erdjument-Bromage H, et al. mTOR interacts with raptor to form a nutrient-sensitive complex that signals to the cell growth machinery. Cell. 2002;110(2):163–75. pmid:12150925.
- 58. Hara K, Maruki Y, Long X, Yoshino K, Oshiro N, Hidayat S, et al. Raptor, a binding partner of target of rapamycin (TOR), mediates TOR action. Cell. 2002;110(2):177–89. pmid:12150926.
- 59. Loewith R, Jacinto E, Wullschleger S, Lorberg A, Crespo JL, Bonenfant D, et al. Two TOR complexes, only one of which is rapamycin sensitive, have distinct roles in cell growth control. Mol Cell. 2002;10(3):457–68. pmid:12408816.
- 60. Stocker H, Radimerski T, Schindelholz B, Wittwer F, Belawat P, Daram P, et al. Rheb is an essential regulator of S6K in controlling cell growth in Drosophila. Nat Cell Biol. 2003;5(6):559–65. pmid:12766775.
- 61. Saucedo LJ, Gao X, Chiarelli DA, Li L, Pan D, Edgar BA. Rheb promotes cell growth as a component of the insulin/TOR signalling network. Nat Cell Biol. 2003;5(6):566–71. pmid:12766776.
- 62. Zhang Y, Gao X, Saucedo LJ, Ru B, Edgar BA, Pan D. Rheb is a direct target of the tuberous sclerosis tumour suppressor proteins. Nat Cell Biol. 2003;5(6):578–81. pmid:12771962.
- 63. Saito K, Araki Y, Kontani K, Nishina H, Katada T. Novel role of the small GTPase Rheb: its implication in endocytic pathway independent of the activation of mammalian target of rapamycin. J Biochem. 2005;137(3):423–30. pmid:15809346.
- 64. Sancak Y, Bar-Peled L, Zoncu R, Markhard AL, Nada S, Sabatini DM. Ragulator-Rag complex targets mTORC1 to the lysosomal surface and is necessary for its activation by amino acids. Cell. 2010;141(2):290–303. pmid:20381137
- 65. Gao X, Pan D. TSC1 and TSC2 tumor suppressors antagonize insulin signaling in cell growth. Genes Dev. 2001;15(11):1383–92. pmid:11390358
- 66. Potter CJ, Pedraza LG, Xu T. Akt regulates growth by directly phosphorylating Tsc2. Nat Cell Biol. 2002;4(9):658–65. pmid:12172554.
- 67. Inoki K, Li Y, Zhu T, Wu J, Guan KL. TSC2 is phosphorylated and inhibited by Akt and suppresses mTOR signalling. Nat Cell Biol. 2002;4(9):648–57. pmid:12172553.
- 68. Sancak Y, Thoreen CC, Peterson TR, Lindquist RA, Kang SA, Spooner E, et al. PRAS40 is an insulin-regulated inhibitor of the mTORC1 protein kinase. Mol Cell. 2007;25(6):903–15. pmid:17386266.
- 69. Vander Haar E, Lee SI, Bandhakavi S, Griffin TJ, Kim DH. Insulin signalling to mTOR mediated by the Akt/PKB substrate PRAS40. Nat Cell Biol. 2007;9(3):316–23. pmid:17277771.
- 70. Pallares-Cartes C, Cakan-Akdogan G, Teleman AA. Tissue-specific coupling between insulin/IGF and TORC1 signaling via PRAS40 in Drosophila. Dev Cell. 2012;22(1):172–82. pmid:22264732.
- 71. Menon S, Dibble CC, Talbott G, Hoxhaj G, Valvezan AJ, Takahashi H, et al. Spatial control of the TSC complex integrates insulin and nutrient regulation of mTORC1 at the lysosome. Cell. 2014;156(4):771–85. pmid:24529379
- 72. Dibble CC, Cantley LC. Regulation of mTORC1 by PI3K signaling. Trends Cell Biol. 2015;25(9):545–55. pmid:26159692
- 73. Dong J, Pan D. Tsc2 is not a critical target of Akt during normal Drosophila development. Genes Dev. 2004;18(20):2479–84. pmid:15466161
- 74. Kockel L, Kerr KS, Melnick M, Bruckner K, Hebrok M, Perrimon N. Dynamic switch of negative feedback regulation in Drosophila Akt-TOR signaling. PLoS Genet. 2010;6(6):e1000990. pmid:20585550
- 75. Saxton RA, Sabatini DM. mTOR Signaling in Growth, Metabolism, and Disease. Cell. 2017;169(2):361–71. pmid:28388417.
- 76. Paradis S, Ruvkun G. Caenorhabditis elegans Akt/PKB transduces insulin receptor-like signals from AGE-1 PI3 kinase to the DAF-16 transcription factor. Genes Dev. 1998;12(16):2488–98. pmid:9716402
- 77. Puig O, Marr MT, Ruhf ML, Tjian R. Control of cell number by Drosophila FOXO: downstream and feedback regulation of the insulin receptor pathway. Genes Dev. 2003;17(16):2006–20. pmid:12893776
- 78. Kramer JM, Davidge JT, Lockyer JM, Staveley BE. Expression of Drosophila FOXO regulates growth and can phenocopy starvation. BMC Dev Biol. 2003;3:5. pmid:12844367
- 79. Junger MA, Rintelen F, Stocker H, Wasserman JD, Vegh M, Radimerski T, et al. The Drosophila forkhead transcription factor FOXO mediates the reduction in cell number associated with reduced insulin signaling. J Biol. 2003;2(3):20. pmid:12908874
- 80. Nowak K, Gupta A, Stocker H. FoxO restricts growth and differentiation of cells with elevated TORC1 activity under nutrient restriction. PLoS Genet. 2018;14(4):e1007347. pmid:29677182
- 81. Fruman DA, Chiu H, Hopkins BD, Bagrodia S, Cantley LC, Abraham RT. The PI3K Pathway in Human Disease. Cell. 2017;170(4):605–35. pmid:28802037
- 82. Huang J, Wu S, Barrera J, Matthews K, Pan D. The Hippo signaling pathway coordinately regulates cell proliferation and apoptosis by inactivating Yorkie, the Drosophila Homolog of YAP. Cell. 2005;122(3):421–34. pmid:16096061.
- 83. Oh H, Irvine KD. In vivo regulation of Yorkie phosphorylation and localization. Development. 2008;135(6):1081–8. pmid:18256197
- 84. Oh H, Irvine KD. In vivo analysis of Yorkie phosphorylation sites. Oncogene. 2009;28(17):1916–27. pmid:19330023
- 85. Wu S, Liu Y, Zheng Y, Dong J, Pan D. The TEAD/TEF family protein Scalloped mediates transcriptional output of the Hippo growth-regulatory pathway. Dev Cell. 2008;14(3):388–98. pmid:18258486.
- 86. Koontz LM, Liu-Chittenden Y, Yin F, Zheng Y, Yu J, Huang B, et al. The Hippo effector Yorkie controls normal tissue growth by antagonizing scalloped-mediated default repression. Dev Cell. 2013;25(4):388–401. pmid:23725764
- 87. Thompson BJ, Cohen SM. The Hippo pathway regulates the bantam microRNA to control cell proliferation and apoptosis in Drosophila. Cell. 2006;126(4):767–74. pmid:16923395.
- 88. Fletcher GC, Diaz-de-la-Loza MD, Borreguero-Munoz N, Holder M, Aguilar-Aragon M, Thompson BJ. Mechanical strain regulates the Hippo pathway in Drosophila. Development. 2018;145(5):dev159467. pmid:29440303.
- 89. Pan Y, Alegot H, Rauskolb C, Irvine KD. The dynamics of hippo signaling during Drosophila wing development. Development. 2018;145(20):dev165712. pmid:30254143.
- 90. Strassburger K, Tiebe M, Pinna F, Breuhahn K, Teleman AA. Insulin/IGF signaling drives cell proliferation in part via Yorkie/YAP. Dev Biol. 2012;367(2):187–96. pmid:22609549.
- 91. Dupont S, Morsut L, Aragona M, Enzo E, Giulitti S, Cordenonsi M, et al. Role of YAP/TAZ in mechanotransduction. Nature. 2011;474(7350):179–83. pmid:21654799.
- 92. Wada K, Itoga K, Okano T, Yonemura S, Sasaki H. Hippo pathway regulation by cell morphology and stress fibers. Development. 2011;138(18):3907–14. pmid:21831922.
- 93. Kim NG, Gumbiner BM. Adhesion to fibronectin regulates Hippo signaling via the FAK-Src-PI3K pathway. J Cell Biol. 2015;210(3):503–15. pmid:26216901
- 94. Pan Y, Heemskerk I, Ibar C, Shraiman BI, Irvine KD. Differential growth triggers mechanical feedback that elevates Hippo signaling. Proc Natl Acad Sci U S A. 2016;113(45):E6974–E6983. pmid:27791172.
- 95. Benham-Pyle BW, Pruitt BL, Nelson WJ. Cell adhesion. Mechanical strain induces E-cadherin-dependent Yap1 and beta-catenin activation to drive cell cycle entry. Science. 2015;348(6238):1024–7. pmid:26023140
- 96. Parker J, Struhl G. Scaling the Drosophila Wing: TOR-Dependent Target Gene Access by the Hippo Pathway Transducer Yorkie. PLoS Biol. 2015;13(10):e1002274. pmid:26474042
- 97. Hsu TH, Yang CY, Yeh TH, Huang YC, Wang TW, Yu JY. The Hippo pathway acts downstream of the Hedgehog signaling to regulate follicle stem cell maintenance in the Drosophila ovary. Sci Rep. 2017;7(1):4480. pmid:28667262
- 98. Chen HJ, Wang CM, Wang TW, Liaw GJ, Hsu TH, Lin TH, et al. The Hippo pathway controls polar cell fate through Notch signaling during Drosophila oogenesis. Dev Biol. 2011;357(2):370–9. pmid:21781961.
- 99. Yu J, Pan D. Validating upstream regulators of Yorkie activity in Hippo signaling through scalloped-based genetic epistasis. Development. 2018;145(4):dev157545. pmid:29467233.
- 100. Zhang L, Ren F, Zhang Q, Chen Y, Wang B, Jiang J. The TEAD/TEF family of transcription factor Scalloped mediates Hippo signaling in organ size control. Dev Cell. 2008;14(3):377–87. pmid:18258485
- 101. Goulev Y, Fauny JD, Gonzalez-Marti B, Flagiello D, Silber J, Zider A. SCALLOPED interacts with YORKIE, the nuclear effector of the hippo tumor-suppressor pathway in Drosophila. Curr Biol. 2008;18(6):435–41. pmid:18313299.
- 102. Ren F, Zhang L, Jiang J. Hippo signaling regulates Yorkie nuclear localization and activity through 14-3-3 dependent and independent mechanisms. Dev Biol. 2010;337(2):303–12. pmid:19900439
- 103. LaFever L, Drummond-Barbosa D. Direct control of germline stem cell division and cyst growth by neural insulin in Drosophila. Science. 2005;309(5737):1071–3. pmid:16099985.
- 104. Burn KM, Shimada Y, Ayers K, Lu F, Hudson AM, Cooley L. Somatic insulin signaling regulates a germline starvation response in Drosophila egg chambers. Dev Biol. 2015;398(2):206–17. pmid:25481758
- 105. Colombani J, Bianchini L, Layalle S, Pondeville E, Dauphin-Villemant C, Antoniewski C, et al. Antagonistic actions of ecdysone and insulins determine final size in Drosophila. Science. 2005;310(5748):667–70. pmid:16179433.
- 106. Stocker H, Hafen E. Genetic control of cell size. Curr Opin Genet Dev. 2000;10(5):529–35. pmid:10980431.
- 107. Djiane A, Zaessinger S, Babaoglan AB, Bray SJ. Notch inhibits Yorkie activity in Drosophila wing discs. PLoS ONE. 2014;9(8):e106211. pmid:25157415
- 108. Brook WJ, Diaz-Benjumea FJ, Cohen SM. Organizing spatial pattern in limb development. Annu Rev Cell Dev Biol. 1996;12:161–80. pmid:8970725.
- 109. Lawrence PA, Struhl G. Morphogens, compartments, and pattern: lessons from drosophila? Cell. 1996;85(7):951–61. pmid:8674123.
- 110. Shraiman BI. Mechanical feedback as a possible regulator of tissue growth. Proc Natl Acad Sci U S A. 2005;102(9):3318–23. pmid:15728365
- 111. Hufnagel L, Teleman AA, Rouault H, Cohen SM, Shraiman BI. On the mechanism of wing size determination in fly development. Proc Natl Acad Sci U S A. 2007;104(10):3835–40. pmid:17360439
- 112. Aegerter-Wilmsen T, Aegerter CM, Hafen E, Basler K. Model for the regulation of size in the wing imaginal disc of Drosophila. Mech Dev. 2007;124(4):318–26. pmid:17293093.
- 113. Aegerter-Wilmsen T, Smith AC, Christen AJ, Aegerter CM, Hafen E, Basler K. Exploring the effects of mechanical feedback on epithelial topology. Development. 2010;137(3):499–506. pmid:20081194.
- 114. Aegerter-Wilmsen T, Heimlicher MB, Smith AC, de Reuille PB, Smith RS, Aegerter CM, et al. Integrating force-sensing and signaling pathways in a model for the regulation of wing imaginal disc size. Development. 2012;139(17):3221–31. pmid:22833127.
- 115. Romano D, Matallanas D, Weitsman G, Preisinger C, Ng T, Kolch W. Proapoptotic kinase MST2 coordinates signaling crosstalk between RASSF1A, Raf-1, and Akt. Cancer Res. 2010;70(3):1195–203. pmid:20086174
- 116. Matallanas D, Romano D, Al-Mulla F, O’Neill E, Al-Ali W, Crespo P, et al. Mutant K-Ras activation of the proapoptotic MST2 pathway is antagonized by wild-type K-Ras. Mol Cell. 2011;44(6):893–906. pmid:22195963.
- 117. Romano D, Maccario H, Doherty C, Quinn NP, Kolch W, Matallanas D. The differential effects of wild-type and mutated K-Ras on MST2 signaling are determined by K-Ras activation kinetics. Mol Cell Biol. 2013;33(9):1859–68. pmid:23459937
- 118. Romano D, Nguyen LK, Matallanas D, Halasz M, Doherty C, Kholodenko BN, et al. Protein interaction switches coordinate Raf-1 and MST2/Hippo signalling. Nat Cell Biol. 2014;16(7):673–84. pmid:24929361.
- 119. Peng XD, Xu PZ, Chen ML, Hahn-Windgassen A, Skeen J, Jacobs J, et al. Dwarfism, impaired skin development, skeletal muscle atrophy, delayed bone development, and impeded adipogenesis in mice lacking Akt1 and Akt2. Genes Dev. 2003;17(11):1352–65. pmid:12782654
- 120. DiGiovanni J, Bol DK, Wilker E, Beltran L, Carbajal S, Moats S, et al. Constitutive expression of insulin-like growth factor-1 in epidermal basal cells of transgenic mice leads to spontaneous tumor promotion. Cancer Res. 2000;60(6):1561–70. pmid:10749124.
- 121. Wilker E, Lu J, Rho O, Carbajal S, Beltran L, DiGiovanni J. Role of PI3K/Akt signaling in insulin-like growth factor-1 (IGF-1) skin tumor promotion. Mol Carcinog. 2005;44(2):137–45. pmid:16086373.
- 122. Sadagurski M, Yakar S, Weingarten G, Holzenberger M, Rhodes CJ, Breitkreutz D, et al. Insulin-like growth factor 1 receptor signaling regulates skin development and inhibits skin keratinocyte differentiation. Mol Cell Biol. 2006;26(7):2675–87. pmid:16537911
- 123. Liu JP, Baker J, Perkins AS, Robertson EJ, Efstratiadis A. Mice carrying null mutations of the genes encoding insulin-like growth factor I (Igf-1) and type 1 IGF receptor (Igf1r). Cell. 1993;75(1):59–72. pmid:8402901.
- 124. Baker J, Liu JP, Robertson EJ, Efstratiadis A. Role of insulin-like growth factors in embryonic and postnatal growth. Cell. 1993;75(1):73–82. pmid:8402902.
- 125. Di Cristofano A, Pesce B, Cordon-Cardo C, Pandolfi PP. Pten is essential for embryonic development and tumour suppression. Nat Genet. 1998;19(4):348–55. pmid:9697695.
- 126. Elbediwy A, Vincent-Mistiaen ZI, Spencer-Dene B, Stone RK, Boeing S, Wculek SK, et al. Integrin signalling regulates YAP and TAZ to control skin homeostasis. Development. 2016;143(10):1674–87. pmid:26989177
- 127. Vincent-Mistiaen Z, Elbediwy A, Vanyai H, Cotton J, Stamp G, Nye E, et al. YAP drives cutaneous squamous cell carcinoma formation and progression. Elife. 2018;7:e33304. pmid:30231971
- 128. Schlegelmilch K, Mohseni M, Kirak O, Pruszak J, Rodriguez JR, Zhou D, et al. Yap1 acts downstream of alpha-catenin to control epidermal proliferation. Cell. 2011;144(5):782–95. pmid:21376238
- 129. Zhang H, Pasolli HA, Fuchs E. Yes-associated protein (YAP) transcriptional coactivator functions in balancing growth and differentiation in skin. Proc Natl Acad Sci U S A. 2011;108(6):2270–5. pmid:21262812
- 130. Debaugnies M, Sanchez-Danes A, Rorive S, Raphael M, Liagre M, Parent MA, et al. YAP and TAZ are essential for basal and squamous cell carcinoma initiation. EMBO Rep. 2018;19(7):e45809. pmid:29875149
- 131. Fan R, Kim NG, Gumbiner BM. Regulation of Hippo pathway by mitogenic growth factors via phosphoinositide 3-kinase and phosphoinositide-dependent kinase-1. Proc Natl Acad Sci U S A. 2013;110(7):2569–74. pmid:23359693
- 132. Lopez-Schier H, St Johnston D. Delta signaling from the germ line controls the proliferation and differentiation of the somatic follicle cells during Drosophila oogenesis. Genes Dev. 2001;15(11):1393–405. pmid:11390359
- 133. Sun J, Smith L, Armento A, Deng WM. Regulation of the endocycle/gene amplification switch by Notch and ecdysone signaling. J Cell Biol. 2008;182(5):885–96. pmid:18779369
- 134. Rauskolb C, Sun S, Sun G, Pan Y, Irvine KD. Cytoskeletal tension inhibits Hippo signaling through an Ajuba-Warts complex. Cell. 2014;158(1):143–56. pmid:24995985
- 135. Dutta S, Mana-Capelli S, Paramasivam M, Dasgupta I, Cirka H, Billiar K, et al. TRIP6 inhibits Hippo signaling in response to tension at adherens junctions. EMBO Rep. 2018;19(2):337–50. pmid:29222344
- 136. Ibar C, Kirichenko E, Keepers B, Enners E, Fleisch K, Irvine KD. Tension-dependent regulation of mammalian Hippo signaling through LIMD1. J Cell Sci. 2018;131(5):jcs214700. pmid:29440237
- 137. Fletcher GC, Elbediwy A, Khanal I, Ribeiro PS, Tapon N, Thompson BJ. The Spectrin cytoskeleton regulates the Hippo signalling pathway. EMBO J. 2015;34(7):940–54. pmid:25712476
- 138. Nolo R, Morrison CM, Tao C, Zhang X, Halder G. The bantam microRNA is a target of the hippo tumor-suppressor pathway. Curr Biol. 2006;16(19):1895–904. pmid:16949821.
- 139. Neto-Silva RM, de Beco S, Johnston LA. Evidence for a growth-stabilizing regulatory feedback mechanism between Myc and Yorkie, the Drosophila homolog of Yap. Dev Cell. 2010;19(4):507–20. pmid:20951343
- 140. Levayer R, Hauert B, Moreno E. Cell mixing induced by myc is required for competitive tissue invasion and destruction. Nature. 2015;524(7566):476–80. Epub 2015/08/20. pmid:26287461.
- 141. Brakebusch C, Grose R, Quondamatteo F, Ramirez A, Jorcano JL, Pirro A, et al. Skin and hair follicle integrity is crucially dependent on beta 1 integrin expression on keratinocytes. EMBO J. 2000;19(15):3990–4003. pmid:10921880
- 142. Piwko-Czuchra A, Koegel H, Meyer H, Bauer M, Werner S, Brakebusch C, et al. Beta1 integrin-mediated adhesion signalling is essential for epidermal progenitor cell expansion. PLoS ONE. 2009;4(5):e5488. pmid:19424505
- 143. Raghavan S, Bauer C, Mundschau G, Li Q, Fuchs E. Conditional ablation of beta1 integrin in skin. Severe defects in epidermal proliferation, basement membrane formation, and hair follicle invagination. J Cell Biol. 2000;150(5):1149–60. pmid:10974002
- 144. Li P, Silvis MR, Honaker Y, Lien WH, Arron ST, Vasioukhin V. alphaE-catenin inhibits a Src-YAP1 oncogenic module that couples tyrosine kinases and the effector of Hippo signaling pathway. Genes Dev. 2016;30(7):798–811. pmid:27013234
- 145. Si Y, Ji X, Cao X, Dai X, Xu L, Zhao H, et al. Src Inhibits the Hippo Tumor Suppressor Pathway through Tyrosine Phosphorylation of Lats1. Cancer Res. 2017;77(18):4868–80. pmid:28754671.
- 146. Yin F, Yu J, Zheng Y, Chen Q, Zhang N, Pan D. Spatial organization of Hippo signaling at the plasma membrane mediated by the tumor suppressor Merlin/NF2. Cell. 2013;154(6):1342–55. pmid:24012335
- 147. Xiao GH, Beeser A, Chernoff J, Testa JR. p21-activated kinase links Rac/Cdc42 signaling to merlin. J Biol Chem. 2002;277(2):883–6. pmid:11719502.
- 148. Surace EI, Haipek CA, Gutmann DH. Effect of merlin phosphorylation on neurofibromatosis 2 (NF2) gene function. Oncogene. 2004;23(2):580–7. pmid:14724586.
- 149. Rong R, Surace EI, Haipek CA, Gutmann DH, Ye K. Serine 518 phosphorylation modulates merlin intramolecular association and binding to critical effectors important for NF2 growth suppression. Oncogene. 2004;23(52):8447–54. pmid:15378014.
- 150. Kissil JL, Johnson KC, Eckman MS, Jacks T. Merlin phosphorylation by p21-activated kinase 2 and effects of phosphorylation on merlin localization. J Biol Chem. 2002;277(12):10394–9. pmid:11782491.
- 151. Hamaratoglu F, Willecke M, Kango-Singh M, Nolo R, Hyun E, Tao C, et al. The tumour-suppressor genes NF2/Merlin and Expanded act through Hippo signalling to regulate cell proliferation and apoptosis. Nat Cell Biol. 2006;8(1):27–36. pmid:16341207.
- 152. Zhang N, Bai H, David KK, Dong J, Zheng Y, Cai J, et al. The Merlin/NF2 tumor suppressor functions through the YAP oncoprotein to regulate tissue homeostasis in mammals. Dev Cell. 2010;19(1):27–38. pmid:20643348
- 153. Sabra H, Brunner M, Mandati V, Wehrle-Haller B, Lallemand D, Ribba AS, et al. beta1 integrin-dependent Rac/group I PAK signaling mediates YAP activation of Yes-associated protein 1 (YAP1) via NF2/merlin. J Biol Chem. 2017;292(47):19179–97. pmid:28972170.
- 154. Mathew G, Hannan A, Hertzler-Schaefer K, Wang F, Feng GS, Zhong J, et al. Targeting of Ras-mediated FGF signaling suppresses Pten-deficient skin tumor. Proc Natl Acad Sci U S A. 2016;113(46):13156–61. pmid:27799550