Yap reprograms glutamine metabolism to increase nucleotide biosynthesis and enable liver growth.

The Hippo pathway is an important regulator of organ size and tumorigenesis. It is unclear, however, how Hippo signalling provides the cellular building blocks required for rapid growth. Here, we demonstrate that transgenic zebrafish expressing an activated form of the Hippo pathway effector Yap1 (also known as YAP) develop enlarged livers and are prone to liver tumour formation. Transcriptomic and metabolomic profiling identify that Yap1 reprograms glutamine metabolism. Yap1 directly enhances glutamine synthetase (glul) expression and activity, elevating steady-state levels of glutamine and enhancing the relative isotopic enrichment of nitrogen during de novo purine and pyrimidine biosynthesis. Genetic or pharmacological inhibition of GLUL diminishes the isotopic enrichment of nitrogen into nucleotides, suppressing hepatomegaly and the growth of liver cancer cells. Consequently, Yap-driven liver growth is susceptible to nucleotide inhibition. Together, our findings demonstrate that Yap1 integrates the anabolic demands of tissue growth during development and tumorigenesis by reprogramming nitrogen metabolism to stimulate nucleotide biosynthesis.

Introduction

Many signaling pathways have been identified to regulate liver growth during organ development and tumor formation. It is unclear, however, how these signals provide energy and cellular building blocks to enable rapid cell division and organ growth. The Hippo signaling pathway has emerged as an evolutionarily conserved master regulator of organ size and tissue growth[1]. The Hippo kinase cascade regulates the transcriptional co-activator Yap that binds the Tead family of transcription factors to enhance cell proliferation, inhibit cell death and alter cell fate[2]. The Hippo pathway is frequently perturbed in human cancers[3], and many oncogenic pathways feed into the Hippo pathway and sustain growth in a Yap-dependent manner. The molecular mechanisms by which Yap target genes contribute to rapid cell proliferation to increase organ size remain elusive.

Altered cellular metabolism is a hallmark of cancer cells[4]. Several studies have focused attention on the alternate means by which cancer cells produce ATP, including aerobic glycolysis[5] or the anaplerotic use of alternate fuel sources such as glutamine[6]. While the mTOR pathway can enhance de novo synthesis of building blocks and macromolecules required for cell growth[7], it remains unknown whether the Hippo pathway can similarly reprogram cellular metabolism to match the demands for rapid tissue growth.

Here, we investigate zebrafish with hepatocyte-specific transgenic expression of activated yap1 that develop hepatomegaly as larvae and are prone to liver tumor formation as adults. Transcriptomic and metabolomic analyses reveal that Yap1 induces glutamine synthetase (glul) to elevate glutamine levels and stimulate de novo nucleotide biosynthesis. Treatment studies in larval and adult zebrafish demonstrate that inhibition of Glul or nucleotide biosynthesis diminishes Yap-induced liver growth. YAP-dependent regulation of GLUL is required for growth of human liver cancer cells. Our studies define a role for Yap in reprogramming cellular metabolism to fulfill the anabolic requirements for tissue growth and illustrate the therapeutic potential of targeting Yap-driven metabolic alterations.

Results

Hepatocyte-specific overexpression of activated Yap causes hepatomegaly and accelerates DMBA-induced liver tumor formation

To investigate the impact of Yap activation on liver growth in zebrafish larvae, transgenic zebrafish (Tg(−2.8fabp10a:yap1-1β), referred to as lf:Yap, were generated with hepatocyte-specific expression of constitutively active Yap1, homologous to human YAP1S127A (). Liver development was visualized using the Tg(−2.8fabp10a:eGFP) (lf:GFP) hepatocyte reporter line[8]. At 5 days post fertilization (dpf), lf:Yap fish exhibit a 36% increase in liver area () compared to wild-type (WT) siblings. Single-plane illumination confocal microscopy confirmed liver volume enlargement and preservation of gross architectural features of the bi-lobed larval liver in lf:Yap trangenics (). Increased liver size was accompanied by hepatocyte hyperproliferation without significantly enlarged cell size, as determined by histological and fluorescence-activated cell sorting (FACS) analyses (). Enhanced liver size in lf:Yap fish persisted into adulthood at 16 weeks post fertilization (wpf), as quantified by fluorescent liver area () and a two-fold increase in liver-to-body weight ratio (). Histological analysis of lf:Yap fish revealed liver hyperplasia with increased cellularity, cell proliferation, decreased glycogen, and focally elevated bile duct density (). These data demonstrate that Yap induces hepatomegaly and promotes liver hyperplasia in zebrafish.

To examine whether Yap predisposes to neoplasia, juvenile WT and lf:Yap transgenics were exposed to the carcinogen dimethylbenzanthracene (DMBA)[9] (). lf:Yap transgenics formed liver tumors earlier and with greater frequency than WT siblings (), with liver masses occupying the entire abdominal cavity (). Tumor differentiation subtypes ranged from hepatocellular carcinoma (HCC), with occasional foci of sarcomatoid cytology and/or peliosis/spongiosis-hepatis-like change, to cholangiocarcinoma (CCA) (). Ascites was noted in 30% (7/23) of lf:Yap transgenics and 0% (0/5) of WT. These data demonstrate that Yap exerts oncogenic activity enhance chemically induced hepatocarcinogenesis.

Yap alters expression of metabolism-related genes and enhances glul expression

To identify signals responsible for Yap-driven liver hyperplasia, we performed transcriptional profiling in WT and lf:Yap adult livers, revealing a large number of differentially expressed genes (). Gene set enrichment analysis was consistent with a mammalian Hippo signature ()[10]. Intriguingly, gene ontology analysis indicated a relationship to metabolism in 34% of annotated categories (), and ~60% of the top 20 biological processes upregulated by Yap were related to metabolism (). Amongst the most differentially upregulated genes were established Yap targets amotl2, ctgf and cyr61, as well as zebrafish orthologues of glutamine synthetase (GLUL), glula and glulb (). Quantitative PCR (qPCR) verified induction of ctgf, cyr61, amotl2, glula and glulb in lf:Yap livers (). GLUL plays a central role in nitrogen assimilation in the liver by catalyzing the formation of glutamine from glutamate and ammonia. While GLUL expression can be regulated by Wnt activity[11], Wnt targets cyclinD1, axin2 or cd44 were not induced in lf:Yap transgenics (). yap expression, but not taz, was dramatically increased in lf:Yap livers (). Collectively, these results suggest that Yap regulates glutamine metabolism.

Yap transcriptionally upregulates GLUL in an evolutionarily conserved fashion

To determine whether Yap directly influences GLUL expression, chromatin immunoprecipitation (ChIP) on isolated adult zebrafish liver lysates was performed. Yap1 occupancy was enriched at the transcriptional start site (TSS) of the glula promoter as avidly as at ctgf (). Mammalian conservation of Yap-dependent GLUL regulation was demonstrated in, a luciferase reporter assay in HEK-293T cells: constitutively active YAP1S127A enhanced GLUL expression, whereas mutant YAP1 lacking the ability to co-activate TEAD (YAP1S94A) did not equally induce GLUL (). Promoter fragmentation analysis found several regions within the promoter to contribute to the total YAP1-induced activity increase, suggesting several binding sites (). ChIP analysis for YAP1 in HepG2 cells revealed occupation of the GLUL promoter in the region associated with luciferase activation (). To further demonstrate the dependency of GLUL expression on Yap activity, genetic and chemical strategies were utilized: shRNA-mediated knockdown of YAP1 and chemical inhibition with verteporfin[12] in Hep3B and HepG2 liver cancer cell lines reduced GLUL (). Together, these studies demonstrate that direct regulation of GLUL expression by YAP1 is evolutionarily conserved in humans.

Yap reprograms nitrogen metabolism by enhancing GLUL-dependent anabolic assimilation of ammonia for de novo nucleotide biosynthesis

To examine the effect of Yap activation on cellular metabolism, adult WT and lf:Yap livers were subjected to polar steady-state metabolomics analysis by liquid chromatography-based tandem mass spectrometry (LC-MS/MS)[13], determining >250 metabolite profiles. Hierarchical clustering based on metabolite abundance revealed significant changes in steady-state levels of many metabolites (, n=5, p<0.05), including enrichment of metabolites associated with protein biosynthesis, purine and pyrimidine metabolism (). Significantly, lf:Yap livers contained twice the amount of glutamine as WT (. Further, GLUL enzyme activity in lf:Yap liver homogenate was increased 10-fold compared to WTs (), and immunohistochemistry demonstrated uniform overexpression of Glul in lf:Yap hepatocytes and heterogeneous expression in Yap-driven liver tumors (). Ammonia excretion rates were decreased when assessed in vivo in lf:Yap fish, consistent with enhanced nitrogen retention due to the catalytic role of GLUL in the formation of glutamine from glutamate and ammonia (). Similarly, metabolomics analysis detected decreased urea levels in lf:Yap livers ().

To more precisely determine the GLUL-dependent fate of ammonia, liver lysates were incubated with 15N-labelled NH4Cl and ATP with or without the GLUL inhibitor methionine sulfoximine (MSO) (). Glutamine is essential for de novo nucleotide biosynthesis as it provides nitrogen atoms for both purines and pyrimidines: three of five nitrogen atoms present on the purine guanosine are contributed by glutamine (two in the purine ring, and one in the amino group at C-2). Similarly, two of three nitrogen atoms present on the pyrimidine cytosine are contributed by glutamine. Incorporation of 15N into nucleotide precursors was monitored by LC-MS/MS using selected reaction monitoring (SRM) for potential 15N isotopologues and revealed that 15N-labelled isotopologues of guanosine and cytosine were increased in lf:Yap liver lysates (). This response was inhibited by MSO. In contrast, little change was observed in the relative isotopic enrichment of 15N into glutamine or histidine (). These results demonstrate that Yap reprograms nitrogen metabolism by activating GLUL and promoting the incorporation of ammonia-bound nitrogen to form glutamine as a precursor for nucleotide biosynthesis.

GLUL activity and nucleotide biosynthesis contribute to Yap-induced hepatomegaly and the growth of liver cancer cells

Given the dramatic impact of Yap on GLUL expression and nitrogen metabolism, the requirement of GLUL in mediating Yap-induced rapid liver growth was examined utilizing morpholino (MO)-mediated knockdown of glula and glulb (). Yap-induced hepatomegaly at 5 dpf was attenuated in glula/glulb morphants (). To demonstrate potential therapeutic implications, larvae were exposed to MSO from 3-5 dpf, which effectively inhibited GLUL activity () and significantly inhibited Yap-driven hepatomegaly (). Importantly, both glula/glulb knockdown and MSO treatment had no effect on liver size or morphology in WT larvae (). Given the increased relative isotopic enrichment of 15N in nucleotide intermediates in lf:Yap transgenics, consistent with stimulation of nucleotide biosynthesis, we investigated whether inhibitors of purine or pyrimidine biosynthesis impacted Yap-driven hepatomegaly: the purine analogue mycophenolic acid (MPA), which inhibits inosine monophosphate dehydrogenase (IMPDH), significantly suppressed Yap-driven hepatomegaly (). Furthermore, the combined treatment of MSO and MPA had an additive effect on liver size (). Similarly, exposure to the pyrimidine analogue 5-Fluorouracil (5FU), which inhibits thymidylate synthase (TS), also suppressed Yap-driven hepatomegaly, but showed no synergy with MSO (). Interestingly, in each case there was no significant impact on WT liver growth (). To examine the conserved nature of the Yap-GLUL axis, Hep3B and HepG2 human liver cancer cells were cultured in the presence or absence of glutamine (Q), MSO or VP. VP suppressed proliferation of Hep3B cells in full media and caused cytostasis in glutamine-deficient media ( n=3). Interestingly, MSO exposure had no effect on Hep3B cell proliferation in full media, however, in glutamine-deprived conditions, Hep3B cell number decreased significantly ( Similar effects of VP and MSO were observed in HepG2 cells cultured in glutamine-deprived conditions (). Together, these studies suggest that GLUL and nucleotide biosynthesis are conditionally required for rapid cell proliferation in the context of Yap-driven hepatomegaly and liver cancer cell growth.

mTOR pathway is not deregulated by Yap expression or GLUL inhibition, but is required for Yap-induced hepatomegaly

Given the important role of mTOR in stimulating nucleotide biosynthesis to fuel cell growth[7], we examined levels of phospho-Akt (p-Akt, S473), an mTORC2 target, as well as phospho-S6 (p-S6), a substrate of S6K: no significant differences were seen in WT and lf:Yap liver homogenates and histological sections (). Importantly, the mTOR inhibitor Rapamycin (RAPA) completely suppressed p-Akt and p-S6 levels; MSO exposure led to a subtle increase in p-Akt and p-S6 levels (). mTOR pathway activation typically leads to increased cell size[7]. Hepatocyte size was examined by liver cell counts, liver area and cellularity in liver sections from WT and lf:Yap larvae and was unaffected by Yap expression (. To determine whether the mTOR pathway was required for Yap-driven liver growth, WT and lf:Yap larvae were exposed to RAPA with or without MSO, which suppressed Yap-driven liver growth, but did not synergize with MSO (). Together, these experiments demonstrate that Yap does not significantly stimulate the mTOR pathway, however, intact mTOR signaling is necessary for Yap-driven liver growth. Furthermore, the mechanism by which MSO suppresses liver growth is dependent on inhibition of the mTOR pathway.

Yap reprograms the relative isotopic enrichment of nutritional nitrogen into nucleotide biosynthesis in a GLUL-dependent manner to support liver growth

The steady-state metabolomics data indicated that Yap alters nitrogen metabolism, but did not define how nitrogen is utilized in vivo to accelerate tissue growth. To examine the fate of increased glutamine content in lf:Yap transgenics, we developed a feeding methodology for stable isotope labeling in fish to assess relative isotopic enrichment in vivo: 15N-labelled Spirulina gel pellets were prepared to provide a defined and consistent amount of 15N-labelled nutrition. Individual WT and lf:Yap fish were fed twice weekly and maintained in the presence or absence of MSO (twice weekly for 48 hr) for 4 weeks (). Subsequently, liver DNA was extracted and hydrolyzed into nucleotides for analysis () to focus exclusively on the fraction of nitrogen incorporated into nucleotides to synthesize DNA and not on other nucleic acid-containing macromolecules, such as RNA. The DNA of lf:Yap transgenic livers contained significantly higher amounts of 15N-labelled nucleotides than WT, with 3 times as much deoxyinosine, twice as much deoxyguanosine and 65% more deoxyadenosine (). Yap-induced increase in nucleotide biosynthesis was mitigated to baseline levels by MSO. The relative isotopic enrichment reveals that Yap reprograms nitrogen metabolism by stimulating anabolic incorporation of glutamine into nucleotides in a GLUL-dependent manner.

To evaluate functional consequences and potential therapeutic impact of GLUL inhibition on adult liver hyperplasia, fish were exposed to MSO twice weekly over a 4-week period to efficiently inhibit GLUL activity in vivo (). Short-term exposure to MSO (for 48 hr) suppressed hepatocyte proliferation, as examined by quantification of PCNA+ nuclei in histological sections (). Importantly, MSO exposure did not cause cell death as determined by TUNEL staining (). Prolonged MSO treatment significantly reduced hepatomegaly in lf:Yap transgenics (). MSO exposure had no effect on overall morphology and liver size in WT, suggesting that GLUL is conditionally required for accelerated hepatic growth following induction of Yap1. These data show that Yap elevates GLUL activity and augments glutamine production, which is essential for nucleotide biosynthesis and DNA assembly during rapid liver growth.

Discussion

In this study, transgenic zebrafish expressing activated Yap1 in differentiated hepatocytes demonstrated rapid onset of Yap-dependent larval hepatomegaly that persists into adulthood, along with increased susceptibility to carcinogen-induced hepatocarcinogenesis. Combined transcriptomic and metabolomic analyses revealed that Yap reprograms nitrogen metabolism by inducing GLUL and elevating steady-state levels of glutamine available for biosynthetic growth. The transcriptional regulation of GLUL by YAP and its impact on growth is evolutionarily conserved. Therapeutic prevention studies with the GLUL inhibitor MSO determined that elevated GLUL activity and nucleotide biosynthesis contribute to Yap-driven hepatomegaly. Collectively, our data establish that Yap reprograms glutamine metabolism to provide essential cellular building blocks for hepatic growth. Given that the Hippo pathway is frequently deregulated in cancer, targeting the metabolic alterations driven by Yap activation is a highly attractive and rational therapeutic approach.

Murine studies demonstrated that Yap alters liver cell fate, induce hepatomegaly and promote tumorigenesis[14-16]. The downstream mechanisms responsible for Yap-driven organ growth, however, have not been fully elucidated. Using zebrafish and unbiased surveys of gene expression and metabolic changes, we identified that Yap reprograms glutamine metabolism through GLUL induction. This results in enhanced de novo nucleotide biosynthesis to meet the anabolic demands of rapid cell proliferation. GLUL is often overexpressed in human hepatoblastoma[17], hepatocellular adenoma[18] and early stage HCC[19]. Consistent with these observations, Glul expression and activity are upregulated in premalignant Yap-driven livers. Glul has been previously characterized as a Wnt target in perivenous hepatocytes [11]. In contrast, Yap is enriched in a subset of ductal cells during liver homeostasis[16], however, Yap levels are elevated in hepatocytes during liver tumorigenesis[20]. Previous ChIP-seq studies examining YAP and TEAD target genes in MCF7 and embryonic stem cells also showed that Yap binds to the GLUL promoter[21, 22]. The Hippo and Wnt pathways appear to have a complex relationship, acting synergistically[23, 24] and antagonistically[25, 26] in different contexts to regulate gene expression. Given the key role of GLUL in nitrogen metabolism, it is not surprising that Met[27], Gata3[28] and Foxo[29] also regulate GLUL in other contexts. We speculate that GLUL overexpression provides tumor cells with a competitive advantage by fulfilling the biosynthetic demands for rapid cell proliferation.

One key feature of malignancy is altered cellular metabolism. Tumor cells exploit metabolic pathways to increase nutrient uptake and bioenergetic output. Aerobic glycolysis (“Warburg effect”) and glutaminolysis (glutamine catabolism to generate TCA cycle intermediates) are among the best described metabolic changes in cancer[5, 6]. A less appreciated aspect of cancer cell metabolism is the need to rewire carbon and nitrogen flux to generate the building blocks required for the anabolic requirements of rapid cell growth[30]. Growing tissue needs lipids to generate membranes, amino acids for macromolecules and proteins, and nucleotides for DNA and RNA synthesis[31]. Recent studies examining the metabolic profiles of Kras-induced pancreatic cancer[32] and Myc-driven lymphomas[33] have identified a common theme in metabolic reprogramming, namely the production of precursors for nucleotide biosynthesis. Here, we discover that Yap reprograms glutamine metabolism to enhance nucleotide biosynthesis and fuel liver growth. Our findings support several recent reports that have elegantly shown that GLUL overexpression can promote cancer cell growth in glutamine-deprived conditions by enhancing nucleotide biosynthesis[34, 35]. Our studies are also consistent with recent insights by Vander Heiden and colleagues, who showed that Ras-driven lung tumors are less dependent on glutamine catabolism (glutaminolysis) than cultured cells[36]. Collectively, these studies illustrate the importance of anabolic glutamine utilization for biosynthetic output and cancer cell growth.

Our in vivo relative isotopic enrichment studies enable tracking of nutritional nitrogen in a complex vertebrate organism like very few studies before[36, 37]. Although our studies focused attention on the anabolic utilization of glutamine for nucleotide biosynthesis, elevated glutamine could also contribute to other biosynthetic outputs including protein synthesis, transamination and the hexosamine biosynthesis pathway. Furthermore, we predict that Yap can alter expression of other metabolic enzymes to enhance utilization of nitrogen and carbon and remodel cellular metabolism. In our work, we highlight the therapeutic potential of targeting anabolic glutamine metabolism with MSO. There is a rich history of targeting the metabolic adaptations of cancer cells as a therapeutic strategy. Many of the first cancer drugs were antimetabolites targeting folate and nucleotide biosynthesis[5, 38]. Antifolates such as methotrexate and nucleoside analogues including 5FU, gemcitabine and cytarabine remain a lynchpin of modern chemotherapy in many cancers. Indeed, we found that Yap-driven liver growth was sensitive to the nucleoside analogues MPA and 5FU. The ability to convert nutrients into biomass is an essential characteristic of tumors that may provide a therapeutic window for novel antimetabolite strategies.

Functional crosstalk between the mTOR and Hippo pathways during tissue growth is well described[39]. The mTOR pathway is essential in linking nutrient status with metabolic processes underlying anabolic cell growth[7]. Intracellular nutrients activate mTOR, altering metabolic flux to generate the lipids, protein and nucleic acids for cell proliferation. For example, the mTOR pathway phosphorylates and thereby activates CAD, which catalyzes the first three steps of pyrimidine biosynthesis[40, 41]. mTOR also stimulates purine biosynthesis by inducing enzymes associated with the mitochondrial tetrahydrofolate cycle[42]. Similarly, lysophosphatidic acid, sphingosine 1-phosphate and the mevalonate pathway regulate Yap, thereby establishing Yap as a sensor of nutrient status [43-46]. Serum starvation activates Amot130, which binds Yap and facilitates its degradation by recruiting E3 ubiquitin ligase Aip4[47, 48]. In the context of liver growth, bile acids derived from mevalonate precursors activate Yap to promote carcinogenesis[49]. In addition to serum-borne lipids, glucose deprivation and bioenergetic stress inhibit Yap activation via AMPK and LATS1/2[50-53]. In turn, Yap directly induces the expression of amino acid transporters SLC38A1 and SLC7A5, which are required for cancer cell growth as they stimulate amino acid uptake and activate mTORC1[54, 55]. In light of these studies and the insights provided by our work, we hypothesize that Yap functions to “sense” the nutrient status of the environment and initiate an appropriate growth response. Given the striking similarities between the mTOR and Hippo pathways as networks that integrate metabolite availability to anabolic growth, it will be interesting to further define these links in the context of cancer.

In summary, our study provides compelling evidence that metabolic reprogramming contributes to the accelerated growth phenotype imbued by Yap activation. A greater understanding of the metabolic perturbations specific to malignant cells may provide new pharmacological approaches to combat cancer.

Online Methods

Zebrafish Husbandry

Zebrafish were maintained according to institutional animal care and use committee (IACUC-BIDMC) protocols. Lines used in this study include WT (AB) and Tg(−2.8fabp10a:eGFP)as3, abbreviated lf:GFP[56]. Tg(−2.8fabp10a:yap1), abbreviated lf:Yap, were generated using standard techniques[57]. These zebrafish express a constitutively active form of yap1-1β, a kind gift from Ian Scott, driven by the hepatocyte-specific promoter of fatty acid binding protein (fabp) 10a, otherwise known as liver specific fatty acid binding protein (lfabp or lf)[. This line also contains the A-crystallin (cryaa)-driven selection marker Venus[58], to produce green fluorescence in the lens of the eye. Adult zebrafish were used without sex bias (both males and females, in a gender-matched fashion), unless otherwise indicated. For the adult zebrafish studies, at least 3 individuals were used for all assays and the age of the individuals examined was 3-months old (unless otherwise stated in the text).

Chemical Exposure

Zebrafish were exposed to methionine sulfoximine (MSO, 1 mM), mycophenolic acid (MPA, 10 μM), 5-Fluorouracil (5FU, 10 μM) and Rapamycin (RAPA, 0.5 μM) as described. Cultured cells were exposed to Verteporfin (VP, 5 μM) and MSO 1 mM), as described. Where necessary, chemicals were dissolved in DMSO. Chemicals were obtained from Sigma-Aldrich (USA).

Morpholino Injection

Morpholinos (MO) (GeneTools USA) designed against exon2-intron2 splice sites of glula and glulb or mismatched controls glula-MM and glulb-MM (see Supplementary Table 1) were injected into Tg(−2.8fabp10a:eGFP) and Tg(−2.8fabp10a:eGFP); lf:Yap larvae at the one-cell-stage.

Fluorescence determination of liver size

lf:GFP larvae were anesthetized with 0.04 mg/ml tricaine methane sulfonate (MS-222) and imaged by fluorescence microscopy using a Zeiss Discovery V8/Axio Cam MRC. Lightsheet microscopy was performed using a Zeiss Lightsheet Z.1 at the Harvard Center for Biological Imaging (HCBI) core and analyzed using FIJI (NIH) as previously described[59].

Histology

Paraformaldehyde (PFA)-fixed larvae, fish were paraffin-embedded, serially sectioned and stained with Hematoxylin and Eosin (H&E), Periodic Acid-Schiff (PAS) or Sirius Red stain using standard protocols[60]. Analysis of PCNA+ nuclei and cellularity (cells/unit2) was performed using FIJI (NIH) as previously described[59].

Immunohistochemistry

Fixed tissue embedded in paraffin was serially sectioned prior to immunohistochemical analysis. Slides were deparaffinized and rehydrated prior to heat-induced antigen retrieval. Antigens were detected using primary antibodies (Supplementary Table 2) in conjunction with an HRP/DAB (ABC) detection kit (Abcam, ab64264) or fluorophore-conjugated secondary antibodies. TUNEL staining was performed according to the manufacturers instructions (R&D Systems).

FACS Analysis

lf:GFP larvae were dissociated at 10 dpf by enzymatic disaggregation in TrypLETM Express (Invitrogen, CO, USA) combined with manual disruption using a pestle. Upon addition of DMEM with 10% FCS, cells were strained through a 35μm nylon mesh and analyzed using a BD FACSAria II flow cytometer (BD Biosciences).

DMBA-induced carcinogenesis

WT and lf:Yap fry were exposed to 5 ppm DMBA for 24 hrs at 3, 4 and 5 weeks[9]. Fish were monitored closely for tumor development over the subsequent 6 months.

RNA Transcriptomic Analysis

RNA was extracted in Trizol (Life Technologies) from livers isolated from WT and lf:Yap adults and purified using the RNease Mini Kit (Qiagen), according to the manufacturers instructions. RNA quality was checked by Agilent Bioanalyzer Sequencing was performed after library construction on an Illumina HiSeq. polyA sequence data were aligned on to the ZV9 genomic assembly using STAR and differentially affected genes were identified using DeSeq[61]. Gene ontology (GO) and Gene Set Enrichment analysis (GSEA) of biological processes was determined by GO Slim (Gene Ontology Consortium) and GAGE[62].

qRT-PCR

RNA was isolated from pooled zebrafish larvae or isolated livers using Trizol. Following DNAse treatment, cDNA was synthesized using the SuperScript III First-Strand Synthesis kit (Life Technologies). qRT-PCR was performed on biological triplicates using an iCycler with iQ SYBR green (BioRad). Gene expression was analyzed with ef1a as the reference gene (Supplementary Table 1). All of the primers used in this study were purchased from Integrated DNA Technologies (Coralville, IA).

ChIP analysis

Chromatin Immunoprecipitation was performed as previously described[63]. Cells were cross-linked in 1% formaldehyde for 10min at room temperature after which the reaction was stopped by addition of 0.125M glycine. Cells were lysed and harvested in ChIP buffer (100 mM Tris at pH 8.6, 0.3% SDS, 1.7% Triton X-100, and 5 mM EDTA) and the chromatin disrupted by sonication using a Diagenode Bioruptor sonicator UCD-200 to obtain fragments of average 200-500 bp in size. Suitable amounts of chromatin were incubated with specific antibodies overnight (Supplementary Table 2). Immunoprecipitated complexes were recovered on Protein-A/G agarose beads (Pierce) and, after extensive washes; DNA was recovered by reverse crosslinking and purification using QIAquick PCR purification kit (QIAGEN).

Cell lines

No cell lines used in this study were found in the database of commonly misidentified cell lines that is maintained by ICLAC and NCBI Biosample. Cell lines were purchased from ATCC just prior to commencing the experiments. The cell lines were not authenticated and were not tested for mycoplasma contamination.

Luciferase assay

Hek293T cells were obtained from American Type Culture Collection (ATCC) and maintained in Dulbecco's Modified Eagle Medium (DMEM; Cellgro) supplemented with 10% FBS (Gibco). Cells were maintained at 37°C in a humidified atmosphere with 5% CO2. HEK293T cells were co-transfected with glutamine synthetase reporter constructs[29], the Renilla plasmid, and mutant isoforms of yap[64, 65], including pCMV-Yap1-2α-S127A (Addgene, #17794), or pCMV-Yap1-2α-S94A (Addgene, #33102). pCMV-EGFP (Addgene, #11153) was used as control. Cells were harvested 48 hrs after transfection using the Dual-Glo Luciferase Assay System (Promega) and assayed according to the manufacturer's directions.

Yap knockdown in liver cancer cell lines

HepG2 and Hep3B cells were obtained from ATCC and maintained in Minimum Essential Medium (MEM; Cellgro) with Earle's salts and L-glutamine supplemented with 10% fetal bovine serum. Cells were maintained at 37°C in a humidified atmosphere with 5% CO2. For shRNA silencing of Yap a single-stranded oligonucleotide encoding Yap target shRNA, and its complement, were synthesized (Supplementary Table 1). The oligonucleotide sense and antisense pair was annealed and inserted into the pLKO.1 backbone. To produce lentiviral supernatents, HEK293T cells were cotransfected with control or shRNA-containing pLKO.1 vectors, VSVG and psPAX2 for 48 hours. HepG2 and Hep3B cells at approximately 40% confluence were infected with lentiviral particles for 24 hrs followed by selection in 2 μg/mL puromycin for 48 hrs prior to cell lysis.

Liver cancer cell line growth assay

HepG2 and Hep3B cells were seeded in 96 well plates in MEM containing Earle's salts and L-glutamine supplemented with 10% fetal bovine serum. Twenty-four hours after seeding, cells were washed with PBS and incubated in MEM media containing 10% dialyzed fetal bovine serum (Gibco), with or without L-glutamine. Where appropriate media was supplemented with 1 mM MSO or 10 μM verteporfin. Cell proliferation was monitored using the Sulforhodamine B (SRB) assay. Adherent cells were fixed by addition of 12.5% (w/v) trichloroacetic acid and incubation at 4°C for 1 hour. Wells were washed with water and cells were stained by addition of WRB solution (0.5% (w/v) SRB in 1% acetic acid). Wells were washed twice with 1% acetic acid and allowed to dry at room temperature. SRB was solubilized with 10 mM Tris, pH 10.5 and absorbance at 510 nm was measured.

Immunoblot analysis

Cell lysates were prepared using RIPA buffer, resolved by SDS-PAGE and electrophoretically transferred onto nitrocellulose. Membranes were probed with the primary antibody overnight and detected with secondary antibody conjugated with HRP (Supplementary Table 2). Antibody complexes were visualized by enhanced chemiluminescence using X-ray film.

Steady-state Metabolomics Analysis

Livers were isolated from adult WT and lf:Yap transgenic adults and a methanol extraction was performed. Polar metabolites were isolated and enriched using the methodology outlined by Yuan et al[13]. Metabolite fractions were collected and analyzed by targeted LC-MS/MS via selected reaction monitoring (SRM) with positive/negative ion polarity switching using a 5500 QTRAP hybrid triple quadrupole mass spectrometer (A/B SCIEX). Metabolic pathway enrichment analysis was performed using MetaboAnalyst[66].

GLUL activity assay

Glul activity was assayed using the γ-glutamyltransferase assay as previously described[67]. Briefly, WT and lf:Yap transgenic larvae or adult livers were lysed in 50 mM imidazole and samples were purified using micro bio-spin gel p-6 columns (BioRad). Lysates were incubated in activity buffer (50 mM imidazole, 50 mM L-glutamine, 25 mM hydroxylamine, 25 mM sodium arsenate, 2mM manganese chloride, 0.16 mM adenosine diphosphate) at 27 °C for 30 min. The reactions were quenched in stop solution (2.42% iron chloride and 1.45% trichloroacetic acid in 1.82 N hydrochloric acid). Absorbance was read at 520 nm and a calibration curve of glutamyl-γ-hydroxamate (Sigma) was used to calculate nmol of product formed.

Determination of ammonia excretion rate

The rate of ammonia excretion was determined by placing individual fish into small water containers and monitoring ammonia buildup over time using methods previously established[68] and an ammonia detection kit (Biovision Inc.) according to the manufacturers instructions.

Analysis of the relative isotopic enrichment in liver lysates following 15NH4Cl exposure

Ammonia incorporation into nucleotide precursors was measured using adaptations to previously established methods[69]. Briefly, liver homogenates isolated from WT and lf:Yap adults were prepared in lysis buffer (100mM NaCl, 25mM Imidazole, 25mM HEPES, 1mM MgCl2, 1mM MnCl2, 0.1mM KCl and 1% NP-40 pH 7.4 supplemented with Complete protease inhibitors (Roche)). Liver homogenates (90 μl) containing the same amount of protein were incubated a reaction cocktail (10 μl) containing 10 mM 15NH4Cl (Cambridge Isotopes Laboratories, Inc.), 10 mM ATP and 10 mM sodium glutamate and incubated at 37 °C for 20 min before the reaction was quenched in 80% methanol (900μl). Polar metabolites were enriched using the methodology outlined by Yuan et al[13] and quantified using SRM on a 5500 QTRAP mass spectrometer using a protocol to detect 15N-labelled isotopologues of nucleotide precursors (Supplementary Table 3).

15N-Spirulina feeding protocol

15N-labelled Spirulina (98%) (Cambridge Isotopes Laboratories, Inc.) gels containing 50 mg/ml 15N-labelled Spirulina, 5 mg/ml Gemma Micro 300 (Skretting) and 1% agar were aliquoted into 30 μl pellets. Individual WT and Tg(fabp10:yap1S87A) transgenic adults were given a 15N-labelled Spirulina gel pellet twice a week over a 4 week period.

Analysis of the relative isotopic enrichment of 15N in genomic DNA

Livers were isolated from adult WT and lf:Yap transgenic adults and genomic DNA was isolated using Quick-gDNA™ MiniPrep (Zymo Research) according to the manufacturers instructions and re-purified by sodium acetate precipitation. DNA from 15N-labelled spirulina and unlabelled spirulina was extracted as previously described[70]. Purified DNA was quantified with PicoGreen (Life Technologies), and 100 ng of DNA was treated with DNA Degradase Plus (Zymo Research) for 24 hrs. Completion of DNAse digestion was measured by PicoGreen quantification. Hydrolyzed nucleotides were enriched using the methodology outlined by Yuan et al[13] and quantified using SRM on a 5500 QTRAP mass spectrometer using a protocol to detect 15N-labelled isotopologues of nucleotides (Supplementary Table 3).

Statistics and Reproducibility

Sample sizes and reproducibility for each figure are denoted in the figure legends. Unless otherwise noted, all data including immunoblots and microscopy images are representative of at least three biologically independent experiments. For zebrafish experiments, no statistical method was used to predetermine sample size. Furthermore, the experiments were not randomized and the Investigators were not blinded to allocation during experiments and outcome assessment. Statistical significance between conditions was assessed by two-tailed Student's t-tests. All error bars represent s.e.m., and significance between conditions is denoted as *p<0.05; **p<0.01; ***p<0.001 and ****p<0.0001. Raw data from independent replicate experiments can be found in the Statistics Source (Supplementary Table 4). Statistical data for each quantitative experiment, including mean, s.e.m., and exact p values can be found in the Statistics Source Data.