Browse Subject Areas

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

A Role for Drosophila dFoxO and dFoxO 5′UTR Internal Ribosomal Entry Sites during Fasting

  • Eugenia Villa-Cuesta ,

    Affiliation: Department of Ecology and Evolutionary Biology, Brown University, Providence, Rhode Island, United States of America

    Current address: Department of Pediatrics, Brown University and Rhode Island Hospital, Providence, Rhode Island, United States of America

  • Brian T. Sage,

    Affiliation: Department of Ecology and Evolutionary Biology, Brown University, Providence, Rhode Island, United States of America

  • Marc Tatar

    Affiliation: Department of Ecology and Evolutionary Biology, Brown University, Providence, Rhode Island, United States of America

A Role for Drosophila dFoxO and dFoxO 5′UTR Internal Ribosomal Entry Sites during Fasting

  • Eugenia Villa-Cuesta, 
  • Brian T. Sage, 
  • Marc Tatar
  • Published: July 9, 2010
  • DOI: 10.1371/journal.pone.0011521


One way animals may cope with nutrient deprivation is to broadly repress translation by inhibiting 5′-cap initiation. However, under these conditions specific proteins remain essential to survival during fasting. Such peptides may be translated through initiation at 5′UTR Internal Ribosome Entry Sites (IRES). Here we show that the Drosophila melanogaster Forkhead box type O (dFoxO) transcription factor is required for adult survival during fasting, and that the 5′UTR of dfoxO has the ability to initiate IRES-mediated translation in cell culture. Previous work has shown that insulin negatively regulates dFoxO through AKT-mediated phosphorylation while dFoxO itself induces transcription of the insulin receptor dInR, which also harbors IRES. Here we report that IRES-mediated translation of both dFoxO and dInR is activated in fasted Drosophila S2 cells at a time when cap-dependent translation is reduced. IRES mediated translation of dFoxO and dInR may be essential to ensure function and sensitivity of the insulin signaling pathway during fasting.


Changes in nutrient availability produce contrasting physiological states of fasting and feeding. This variation in nutrition is managed at both cellular and systemic levels. One cellular response is to repress the overall level of 5′cap-initiated translation [1][4] as seen in glucose deprived yeast [5], fasted rats [6], [7], and amino acid deprivation in many organisms (reviewed in [8]). Repressing the overall production of proteins is likely to reduce metabolite demands when nutrients are limited, but the synthesis of some proteins is essential for cells to positively adapt to the stress [3].

When deprived of glucose, yeast cells appear to maintain some proteins by translation initiation at Internal Ribosomal Entry Sites (IRES) within the 5′ UTR [5]. While IRES are best described in viral mRNA [9], [10], cellular IRES have been described in a limited but increasing number of mRNAs [1], [11] [See IRES database (​tabase/]. The function of IRES in these cellular mRNAs has remained elusive, but their distribution among gene types suggests that IRES-dependent translation allows physiological adaptation to stress [5].

Several genes of the fly Drosophila melanogaster have identified IRES, including the insulin-like receptor dInR [12]. Importantly, the insulin receptor is at the interface between the systemic and cellular response to nutrients [13][16]. As conserved from mammals to Drosophila [17], fasting reduces the circulating level of insulin. Reduced binding of insulin at the insulin-like receptor inhibits the serine-threonine kinase AKT, blocking phosphorylation of dFoxO. dFoxO may then be transported to the nucleus to induce many genes associated with fasting metabolism. Several Drosophila studies suggest dFoxO is an important transcription factor involved in the adaptation to nutrient stress [15], [18]. Global gene expression profiling showed that 28% of genes up-regulated during nutrient deprivation are also induced by expression of constitutively active dFoxO in Drosophila S2 cells [18]. Among these genes are the insulin-like receptor dInR [15], and the translation regulator 4E-BP [19], [20], [21]. This reciprocal connection between dInR post-translational regulation of dFoxO and dFoxO transcriptional control of dInR suggests that this signaling pathway functions as a homeostatic feedback network. It will increase insulin sensitivity by increasing receptor abundance in cells of peripheral tissues when circulating nutrients are low, and decrease insulin sensitivity when nutrients are high.

Here we investigate the role IRES play in the maintenance of the insulin signal transduction pathway during fasting. We show that during fasting, when general levels of translation are reduced, the relative abundance of dFoxO protein increases, and that this increase occurs without changing the level of dfoxO mRNA. We find that the 5′UTR of dfoxO has the ability to initiate IRES-mediated translation, and that dfoxO-IRES translation is active when fasting decreases cap-dependent translation. Furthermore, translation is also initiated at the IRES of dInR in fasting cells. Cap-independent translational control of dFoxO and of dInR may be a molecular mechanism that allows fasting cells to acquire an insulin-sensitive state and thus adapt the cells to respond rapidly to re-feeding.


dFoxO confers survival during fasting

Overexpression of dFoxO in larvae slows growth, inhibits feeding and produces small adults [22]. In adults the role of dFoxO during fasting is ambiguous. Loss of dfoxO reduces the capacity to survive upon amino acid depleted diet [23] although an independent study found dfoxO null flies were insensitive to starvation when measured on the scale of days [24]. To clarify the role of dfoxO during fasting, we studied the survival time of various homozygous null dfoxO flies maintained on media without yeast and sugar. The survival time of null homozygotes (dfoxO21/21) but not of heterozygotes (dfoxO21/+) was reduced by 50% on the nutrient depleted media (Fig. 1A). Null flies of the trans-genotype dfoxO21/dfoxOw24 were likewise sensitive to total nutrient deprivation (Fig. 1B).

Figure 1. Relative dFoxO protein increases and confers survival during fasting.

Null mutants homozygous (A) dfoxO21 and (B) trans-heterozygous dfoxO21/dfoxOw24 have reduced survival during fasting relative to wild type and dfoxO21/+. (C) Sub-cellular localization of dFoxO in decapitated bodies of fed and fasted females. Lysates were analyzed by Western immunoblot for dFoxO, Lamin as nuclear (N) and Hsp90 as cytosolic (C) controls. Numbers indicate the quantification by densitometry to obtain the ratio dFoxO to Lamin in N, or Hsp90 in C. dFoxO nuclear quantification was corrected for contamination by subtracting Hsp90 from nuclear fractions. Likewise, Lamin in the cytosol was subtracted from the dFoxO cytosolic quantifications. The nuclear fraction lane from the fasted samples shows a prominent Hsp90 band that we have considered contamination. However, Hsp90 may translocate to the nucleus upon fasting. In that situation, the ratio dFoxO to Lamin would be higher that 0.8. (D) dfoxO mRNA abundance from decapitated bodies of fed and fasted females flies. Relative gene expression was analyzed by 2−ΔΔCT method [33]. Data are shown as the mean +1 standard deviation. *, P<0.05 versus control.


Relative dFoxO protein increases during fasting

FoxO proteins are post-translationally modified to regulate their localization in response to nutrition [25]. To study dFoxO protein cellular distribution in fasted flies, we examined its localization by western blot analysis of cell fractionated samples from body tissue. Relative to Lamin and Hsp90 controls, levels of dFoxO were elevated in both cytosolic and nuclear compartments in the bodies of fasted flies (Fig. 1C). Additionally, there was a small increase in the level of dfoxo transcripts (Fig. 1D).

dfoxO 5′UTR can initiate IRES-mediated translation

Because cap-dependent translation is decreased when cells and animals are fasted, we looked to see if dFoxO proteins are maintained during fasting through a cap-independent translation mechanism such as IRES translation. mRNAs containing IRES have long 5′UTRs that contain multiple upstream AUG sequences [26]. The dfoxO gene has four unique 5′UTRs; all are relatively long, being greater than the average size of 256 bp in Drosophila [27], and three dfoxO 5′UTRs contain internal AUGs (Fig. 2A). 5′UTR-A and -E are similar (5′UTR-E has an additional 20 bp located at the 5′ end). These sequences each contain three upstream ATGs. 5′UTR-B is the longest 5′UTR with 9 upstream ATGs. 5′UTR-C and -D are identical and have no upstream ATG (Fig. 2A).

Figure 2. The dfoxO 5′UTR contains IRES.

(A) Diagram of the genomic region of predicted dfoxO's 5′UTRS. 5′UTR-A and -E are similar (5′UTR-E has an additional 20 bp located at the 5′ end). These sequences each contain three upstream ATGs (location marked as 3*). 5′UTR-B is the longest 5′UTR and with 9 upstream ATGs (location marked as 9*). 5′UTR-C and -D are identical and have no upstream ATG. (B) Scheme of the di-cistronic reporter construct. Enhanced cyan fluorescent protein (eCFP) in blue and enhanced yellow fluorescent protein (eYFP) in green. (C–E) Drosophila S2 cells transfected with eCFP/eYFP di-cistroninc reporter. (C) empty vector (D) vector with dfoxO 5′UTR-A in forward 5′-3′orientation, (E) and vector dfoxO 5′UTR-A in reverse 3′-5′orientation. (F) vector with dfoxO 5′UTR-B in forward 5′-3′orientation, (G) and vector dfoxO 5′UTR-B in reverse 3′-5′orientation. (H) vector with dfoxO 5′UTR-C in forward 5′-3′orientation, (I) and vector dfoxO 5′UTR-C in reverse 3′-5′orientation. The ratios eYFP to eCFP fluorescence are shown above the pictures.


We cloned dfoxO 5′UTR A, B and C between protein-encoding reporter sequences of a di-cistronic construct [28] (Fig. 2D–I). In this construct (Fig. 2B), cap-dependent translation is reported by enhanced cyan fluorescent protein (eCFP). Translation of the second cistron, reported by enhanced yellow fluorescent protein (eYFP), is inefficient unless the cloned UTR contains a functional IRES. Each of these vectors was transfected into Drosophila S2 cells. In cells maintained on nutrient deplete serum free media, only 5′ UTR-B, the longest of dfoxO 5′ UTRs, which contains 9 upstream AUGs (Fig 2A), was able to initiate IRES-mediated translation of eYFP (compare Fig 2D, 2H with 2F). As controls we transfected empty vectors or vectors with the 5′UTRs in reverse orientation. Neither of these controls showed IRES activity (Fig. 2C,E,G,I).

dfoxO-IRES and dInR-IRES translation is active when fasting represses cap-dependent translation in insects cells

The level of dFoxO protein may be preserved in fasted cells if IRES mediated translation is active when cap-dependent translation is repressed. To study dfoxO-IRES mediated translation we cloned dfoxO 5′UTR-B in a second dicistronic construct in which cap-dependent translation is reported by renilla luciferase, while IRES initiated translation is reported by firefly luciferase [12] (Fig. 3A). Cells transfected with the renilla/firefly vector showed similar results to the 5′UTR-B cloned in the eCFP/eYFP vector, and permitted quantitative measurement based on luminescence. Again, as a control, dfoxO IRES translation was inactive with the 5′UTR inserted in reverse orientation (Fig. 3B). The efficiency of dfoxO IRES-mediated translation was similar to that of other established Drosophila IRES: Antennapedia (Antp) and (dInR) (Fig. 3B). Northern blot analysis showed that mRNAs from cells transfected with the renilla/firefly dfoxO 5′UTR-B inserted in forward orientation were similar in size to those with the dfoxO 5′UTR-B in reverse orientation (Fig. 3C).

Figure 3. Translation from dfoxO-IRES and dInR-IRES when fasting represses cap-dependent translation of S2 cells.

(A) Scheme of the di-cistronic reporter construct. Translation from 5′cap is quantified by renilla luminescence. Translation from the IRES of the same cells is quantified from firefly luminescence. (B) Ratio of firefly-to renilla luminescence of dInR-IRES, Antp-IRES and dfoxO-5′UTR-B in forward and reverse orientation. (C) Northern analysis from S2 cells transfected with the di-cistronic renilla-fifefly luciferase reporter with dfoxO-5′UTRB firefly luciferase inserted in forward and reverse orientation. Transfections were done in triplicate. The probe used is specific to firefly luciferase. (D) Ratio of firefly to renilla luminescence of dInR-IRES and dFoxO-5′UTR transfected cells before (0 hours) and after fasting (1 hour). (E) Renilla and firefly luminescence of dInR-IRES and dfoxO-5′UTR in transfected cells before fasting (0 hours) and after fasting (1 hour). Data are shown as the mean +1SD for duplicates determinations. *, P<0.05 versus 0 hrs of fasting.


We starved Drosophila S2 cells transfected with dfoxO 5′UTR inserted in the di-cistronic renilla/firefly construct (Fig. 3D). S2 cells maintained in serum free media are more sensitive to stress than those in complete serum. To avoid cell death, we first determined the maximum time of starvation at which cell viability was maintained. Cells were starved in 1× PBS for 0.5, 1, 2, 4 and 6 hours. 1 hour of starvation did not affect cell viability as measured by trypan blue staining (data not shown).

Cells starved for 1 hour in PBS have increased dfoxO-IRES-mediated translation (firefly) relative to cap-dependent translation (renilla) (Fig 3D). The increased ratio is due to a reduced expression of renilla luciferase while the dfoxO-IRES dependent translation remained constant (Fig 3E). To test if the IRES of dInR shared these behaviors, we studied dInR-IRES translation in starved S2 cells transfected with a dInR-IRES renilla/firefly di-cistronic construct. Similar to dfoxO, the ratio of firefly to renilla luciferase expression increased (Fig. 3C) in fasted cells due to a decrease in cap-dependent translation (Fig. 3E).


FoxO protein is tightly regulated by post-translational modifications including phosphorylation, ubiquitination and acetylation. These regulate its sub-cellular localization, protein stability, DNA binding properties and transcriptional activity [25]. Here we suggest an additional level of control based on the regulation of the initiation of dFoxO translation by IRES.

IRES mediated translation provides yeast cells with proteins needed to cope with starvation [5]. Our data show that under starvation, S2 cells decrease cap-dependent translation as seen by a decrease in the expression of the reporter renilla luciferase, while the reporter for dfoxO IRES dependent translation remains unchanged. This finding suggests that the regulation of dFoxO translation by IRES may help retain essential cellular functions during Drosophila fasting.

dFoxO is required for optimal survival during fasting and dFoxO protein remains constant when the level of total protein decreases in nutrient deprived flies. Based on analysis with S2 cells, this retention of dFoxO protein may in part be explained by IRES mediated translation when cap-dependent translation is otherwise depressed. Previous work has shown that dFoxO protein is dephosphorylated and active in nutrient deprived S2 cells [15], leading to the up-regulation of genes needed for fasting adaptation, such as the translational repressor 4E-BP [19], [20], [21] as well as the insulin receptor itself [15]. Interestingly, our data suggest that in fasted flies, a relative increase in dFoxO protein rather than nuclear translocation is responsible for dFoxO activation (Fig 1C) [25]. Notably, dInR also harbors an IRES [12], and we show that dInR-IRES mediated translation is active in starved S2 cells (Fig. 3). IRES appear to maintain translation of both dInR and dFoxO during nutrient stress in vitro, suggesting that the homeostatic reciprocal relationship between dInR and dFoxO includes not only a mechanism to transcribe the insulin receptor but also a system to ensure production of both dInR and dFoxO proteins. Such a system may also occur in mammals because the concentration of InR protein has been shown to increase substantially in starved HepG2 cells [29]. Our work suggests that the maintenance of InR and FoxO during fasting may ensure there is sufficient FoxO to transcribe genes that are essential for cells to cope with limited nutrients and to increase the potential insulin sensitivity of cells in anticipation of the time when nutrients are again available.

Materials and Methods

Drosophila strains and fasting survival assay

The dfoxO mutants dfoxO21 and dfoxOw24 are described in [30] and [31] respectively. Because the dfoxO21 original stock is homozygote lethal but dfoxO null mutants are homozygous viable [24], [30], we recombined dfoxO21 with yw to eliminate second site mutations and generate homozygous viable lines. Afterward, dfoxO21 and dfoxOw24 stocks were backcrossed to yw for four generations. In all trials yw were used as controls. To assess survival in fasting adults, newly eclosed adult flies were collected within 24 hour. Adults were aged for 4 days under controlled conditions (25°C, 40% relative humidity and 12 h light:12 h dark) on normal media (11% sugar, 2.5% autolyzed yeast, 5.2% cornmeal, agar 0.79% w/v in water and 0.2% tegosep -methyl 4-hydroxybenzoate, from Sigma- St. Louis, MO, USA-). At the age of 5 days, 10 females per vial and 10 vials per genotype were transfered into media for fasting (0.8% agarose w/v in PBS). Dead flies were scored in each vial at 6 hour intervals. Differences among survivorship were assessed by the log rank test [32].

Western Blotting and Cell fractionation

Lysates were generated separately from decapitated bodies of 120 two to four day-old females. Prior to analysis flies were maintained on normal diet or fasting diet for 48 hours. Cytoplasmic and nuclear extracts were prepared from lysed tissues by using the Active Motif Nuclear Extract Kit (Carlsbad, CA. USA, Cat #40010). Total protein concentration was determined using the BCA Protein Assay Kit (Thermo Scientific, Rockford, IL, USA.) following the manufacturers' protocols. For Western blot analysis, 4 µg of total protein per lane were separated using NuPAGE 4–12% Bis-Tris Gel (Invitrogen, Carlsbad, CA, USA.) and electrotransferred to PVDF membrane. Fasted and fed samples were loaded in the same gel. 3 different gels were blotted independently for dFoxO, Lamin and Hsp90. Each membrane was exposed at different times dependently on the antibody- specific antigen recognition.

Antibodies were guinea pig anti-dFoxO (gift from H. Broihier, Case Western Reserve University), mouse anti-Lamin DMO (ADL84.12, Developmental Studies Hybridoma Bank, University of Iowa, Iowa, USA), and rabbit anti-Hsp90 (SPA-846 Stressgen, Ann Arbor, Michigan, USA). Following blotting, the PVDF membranes were stained with Coomassie to verify that equal amounts of protein were transferred. Each experiment was repeated twice.

Quantitative PCR

cDNA was prepared from 25 decapitated bodies from each of three biological samples. Each sample used six to eight day-old yw females that had previously been maintained on a normal or fasting diet for 48 hours. For qPCR, three technical replicates were generated per biological sample. dfoxO mRNA was amplified by the primer pair caatctcgagtgcaatgtcgagga (forward) and ccctgagcatcagcaacattagca (reverse) using Superscript III Platinum SYBR Green One-Step qRT-PCR with ROX (cat. 11746-500, Invitrogen, Carlsbad, CA, USA.) on an ABI 7300 System and standardized against the RPL32 mRNA (forward primer: aatgatgtgcgagtgccgag, reverse primer: caatggtgctgctatcccaatc).

Cloning dfoxO 5′UTR

5′UTR sequences of the dfoxO transcript are described in (Schematic representation in Fig. 2A). To generate the eCFP/eYFP dicistronic construct, the 5′UTR-A, B and C of dfoxO was amplified with the primers aaccatggctagaaagcagttaacgagtagtc (forward) and tttttccatggggtagaaaagttcgttgtgcagt (reverse) from clones LD14524, LD19191 and LD05569 (Berkeley Drosophila Genome Project) respectively. The amplified fragment was subcloned into pNEX3-eCFP –eYFP (provided by John R. Dyer and Wayne S. Sossin [28]) using Nco1sites. The eCFP-5′UTR-eYFP fragment was then PCR amplified with the primers acgcggaattcatggtgagcaagggcgaggagctg (forward) and ttgggcccggtaccttacttgtacagctcgtccatgccg (reverse), and subsequently subcloned into the pAc5.1/V5-HisA vector (Invitrogen) using the EcoRI (5′) and ApaI (3′) sites. To clone this dfoxO 5′UTR into the renilla/firefly di-cistronic construct, the 5′UTR was amplified as before and cloned into the pMARL vector [12] using Nco1 sites.

Renilla-InR-5′UTR-firefly and renilla-Antennapedia-5′UTR-firefly constructs were kindly provided by Michael Marr and Robert Tjian [12].

S2 cell transient transfection

The di-cistronic constructs were transfected into Drosophila S2 cells in serum free media Express Five® SFM (Invitrogen) using Effectene Transfection Reagent (Quiagen, Valencia, CA, USA) following the manufacturer's instructions. Images (objective oil immersion 63×; numeral aperture 1.4) were collected using a Leica TCS SP2 AOBS Confocal Laser Scanning Microscope, 48 hours post-transfection. Samples were mounted in ProLong® Gold antifade reagents (Invitrogen, Carlsbad, CA, USA). Fluorescence was analyzed using the Leica Confocal Software Lite Version. Luciferase activity was measured by using the Dual-Glo™ Luciferase Assay System (Promega) with a SpectraMax M5 microplate reader and SoftMax Pro 4.8. software (Molecular Devices, Sunnyvale, CA, USA.) following the manufacturer's instructions. For starvation assays, 48 hours post-transfection, an equal number of cells from a transfection event were transferred to 1× PBS or media for one hour, and measured for luciferase activity. Three technical replicates were used per treatment. Each transfection was repeated three times. The experiment was repeated twice.

Northern blot analyses

Transfections were performed as described above. RNA was extracted with TRIzol® Reagent following the manufacturer's instructions (Invitrogen, Carlsbad, CA, USA.). Northern blots were conducted with the NorthernMax® Kit following manufacturer's instructions (Ambion, Austin, TX, USA.). Purified RNA (15 µg per lane) was electrophoresed, blotted onto a nylon membrane and probed for firefly luciferase. 32P-labelled probe was synthesized by random primer using the DECAprime™ II kit from Ambiom (Austin, TX, U.S.A) following the manufacturer's instructions.

Statistical analyses

Data are shown as the mean and standard deviation. An unpaired t-test was used for all comparisons. Differences were considered significant at p<0.05. Differences among survivorship were assessed by the log rank test [32].


We thank Heather Broihier for the dFoxO antibody as well as Michael T. Marr, Wayne S. Sossin, and Robert Tjian for the di-cistronic constructs. Also, Ke Ying Wu, Nicola Neretti, Alan Bergland, Rondi Butler, Rochele Yamamoto and other members of the laboratory for advice and discussion; Oscar Puig, Philip Gruppuso, Joan Boylan, Jennifer Sanders and two referees for their helpful comments on the manuscript.

Author Contributions

Conceived and designed the experiments: EVC MT. Performed the experiments: EVC BTS. Analyzed the data: EVC BTS. Wrote the paper: EVC MT.


  1. 1. Holcik M, Sonenberg N (2005) Translational control in stress and apoptosis. Nat Rev Mol Cell Biol 6: 318–327.
  2. 2. Lasko P, Sonenberg N (2007) Coordinated transcriptional and translational control in metabolic homeostasis in flies. Genes Dev 21: 235–237.
  3. 3. Sonenberg N, Hershey JWB, Mathews MB (2000) Translational control of gene expression. Cold Sping Harbor Laboratory Press.
  4. 4. Sonenberg N, Hinnebusch AG (2009) Regulation of translation initiation in eukaryotes: mechanisms and biological targets. Cell 136: 731–745.
  5. 5. Gilbert WV, Zhou K, Butler TK, Doudna JA (2007) Cap-independent translation is required for starvation-induced differentiation in yeast. Science 317: 1224–1227.
  6. 6. Baillie AG, Garlick PJ (1991) Responses of protein synthesis in different skeletal muscles to fasting and insulin in rats. Am J Physiol 260: E891–E896.
  7. 7. McNurlan MA, Tomkins AM, Garlick PJ (1979) The effect of starvation on the rate of protein synthesis in rat liver and small intestine. Biochem J 178: 373–379.
  8. 8. Jefferson LS, Kimball SR (2003) Amino acids as regulators of gene expression at the level of mRNA translation. J Nutr 133: 2046S–2051S.
  9. 9. Pelletier J, Sonenberg N (1988) Internal initiation of translation of eukaryotic mRNA directed by a sequence derived from poliovirus RNA. Nature 334: 320–325.
  10. 10. Jang SK, K Kräusslich HG, Nicklin MJ, Duke GM, Palmenberg AC, et al. (2007) A segment of the 5′ nontranslated region of encephalomyocarditis virus RNA directs internal entry of ribosomes during in vitro translation. J Virol 62: 2636–2643.
  11. 11. Graber TE, Holcik M (2007) Cap-independent regulation of gene expression in apoptosis. Mol Biosyst 3: 825–834.
  12. 12. Marr MT, D'Alessio JA, Puig O, Tijan R (2007) IRES-mediated functional coupling of transcription and translation amplifies insulin receptor feedback. Genes Dev 21: 175–183.
  13. 13. Garofalo RS (2002) Genetic analysis of insulin signaling in Drosophila. Trends Endocrinol Metab 13: 156–162.
  14. 14. Shingleton AW, Das J, Vinicius L, Stern DL (2005) The temporal requirements for insulin signaling during development in Drosophila. PLoS Biol 3: e289.
  15. 15. Puig O, Tjian R (2005) Transcriptional feedback control of insulin receptor by dFOXO/FOXO1. Genes Dev 19: 2435–2446.
  16. 16. Burgering BM (2008) A brief introduction to FOXOlogy. Oncogene 27: 2258–2262.
  17. 17. Accili D, Arden KC (2004) FoxOs at the crossroads of cellular metabolism, differentiation, and transformation. Cell 117: 421–426.
  18. 18. Gershman B, Puig O, Hang L, Peitzsch RM, Tatar M, et al. (2007) High-resolution dynamics of the transcriptional response to nutrition in Drosophila: a key role for dFOXO. Physiol Genomics 29: 24–34.
  19. 19. Teleman AA, Chen YW, Cohen SM (2005) 4E-BP functions as a metabolic brake used under stress conditions but not during normal growth. Genes Dev 19: 1844–1848.
  20. 20. Tettweiler G, Miron M, Jenkins M, Sonenberg N, Lasko PF (2005) Starvation and oxidative stress resistance in Drosophila are mediated through the eIF4E-binding protein, d4E-BP. Genes Dev 19: 1840–1843.
  21. 21. Puig O, Marr MT, Ruhf ML, Tijan R (2003) Control of cell number by Drosophila FOXO: downstream and feedback regulation of the insulin receptor pathway. Genes Dev 17: 2006–2020.
  22. 22. Kramer JM, Davidge JT, Lockyer JM, Staveley BE (2003) Expression of Drosopila FOXO regulates growth and can phenocopy starvation. BMC Dev Biol 3: 5.
  23. 23. Kramer JM, Slade JD, Staveley BE (2008) foxo is required for resistance to amino acid starvation in Drosophila. Genome 51: 668–672.
  24. 24. Giannakou ME, Goss M, Partridge L (2008) Role of dFOXO in lifespan extension by dietary restriction in Drosophila melanogaster: not required, but its activity modulates the response. Aging Cell 7: 187–198.
  25. 25. Salih DA, Brunet A (2008) FoxO transcription factors in the maintenance of cellular homeostasis during aging. Curr Opin Cell Biol 20: 126–136.
  26. 26. van der Velden AW, Thomas AA (1999) The role of the 5′ untranslated region of an mRNA in translation regulation during development. Int J Biochem Cell Biol 31: 87–106.
  27. 27. Misra S, Crosby MA, Mungall CJ, Matthews BB, Campbell KS, et al. (2002) Annotation of the Drosophila melanogaster euchromatic genome: a systematic review. Genome Biol 3: RESEARCH0083.
  28. 28. Dyer JR, Michel S, Lee W, Castellucci VF, Wayne NL, et al. (2003) An activity-dependent switch to cap-independent translation triggered by eIF4E dephosphorylation. Nat Neurosci 6: 219–220.
  29. 29. Hatada EN, McClain DA, Potter E, Ullrich A, Olefsky JM (1989) Effects of growth and insulin treatment on the levels of insulin receptors and their mRNA in Hep G2 cells. J Biol Chem 264: 6741–6747.
  30. 30. Jünger MA, Rintelen F, Stocker H, Wasserman JD, Végh M, et al. (2003) The Drosophila forkhead transcription factor FOXO mediates the reduction in cell number associated with reduced insulin signaling. J Biol 2: 20.
  31. 31. Weber K, Johnson N, Champlin D, Patty A (2005) Many P-element insertions affect wing shape in Drosophila melanogaster. Genetics 169: 1461–1475.
  32. 32. Parmer MKB, Machine D (1995) Survival Analysis: A practical approach. Wiley Chichester.
  33. 33. Livak KJ, Schmittgen TD (2001) Analysis of relative gene expression data using real-time quantitative PCR and the 2(-Delta Delta C(T)) Method. Methods 25: 402–408.