Madm (Mlf1 adapter molecule) cooperates with Bunched A to promote growth in Drosophila
© Gluderer et al.. 2010
Received: 29 August 2009
Accepted: 22 December 2009
Published: 11 February 2010
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© Gluderer et al.. 2010
Received: 29 August 2009
Accepted: 22 December 2009
Published: 11 February 2010
The TSC-22 domain family (TSC22DF) consists of putative transcription factors harboring a DNA-binding TSC-box and an adjacent leucine zipper at their carboxyl termini. Both short and long TSC22DF isoforms are conserved from flies to humans. Whereas the short isoforms include the tumor suppressor TSC-22 (Transforming growth factor-β1 stimulated clone-22), the long isoforms are largely uncharacterized. In Drosophila, the long isoform Bunched A (BunA) acts as a growth promoter, but how BunA controls growth has remained obscure.
In order to test for functional conservation among TSC22DF members, we expressed the human TSC22DF proteins in the fly and found that all long isoforms can replace BunA function. Furthermore, we combined a proteomics-based approach with a genetic screen to identify proteins that interact with BunA. Madm (Mlf1 adapter molecule) physically associates with BunA via a conserved motif that is only contained in long TSC22DF proteins. Moreover, Drosophila Madm acts as a growth-promoting gene that displays growth phenotypes strikingly similar to bunA phenotypes. When overexpressed, Madm and BunA synergize to increase organ growth.
The growth-promoting potential of long TSC22DF proteins is evolutionarily conserved. Furthermore, we provide biochemical and genetic evidence for a growth-regulating complex involving the long TSC22DF protein BunA and the adapter molecule Madm.
See minireview at http://jbiol.com/content/9/1/8.
A prevalent model of carcinogenesis suggests that sequential activation of oncogenes and inactivation of tumor suppressor genes occur in a multistep process leading to deviant growth. Over the past decades much effort has been put into identifying tumor suppressor genes and their pathways because they represent attractive drug targets for cancer therapy. On the basis of expression data derived from various human and murine tumor tissues, Transforming growth factor-β1 stimulated clone-22 (TSC-22) - originally identified as a TGF-β1-responsive gene  - is believed to be a tumor suppressor gene [2–5]. TSC-22 exhibits pro-apoptotic functions in cancer cell lines [6, 7], and a recent study reported that genetic disruption of the TSC-22 gene in mice cause higher proliferation and repopulation efficiency of hematopoietic precursor cells, consistent with a role of TSC-22 in tumor suppression . However, TSC-22 knockout mice do not display enhanced tumorigenesis. Because TSC-22 possesses a leucine zipper and a novel motif capable of binding DNA in vitro - the TSC-box  - TSC-22 is likely to operate as a transcription factor. Alternatively, TSC-22 might act as transcriptional regu-lator as it binds to Smad4 via the TSC-box and modulates the transcriptional activity of Smad4 . Furthermore, Fortilin (TCTP) binds to and destabilizes TSC-22, thereby impeding TSC-22-mediated apoptosis .
Unraveling the precise mechanism by which TSC-22 acts is demanding because there are several mammalian genes homologous to TSC-22 that could have, at least in part, redundant functions. TSC-22 is affiliated with the TSC-22 domain family (TSC22DF) consisting of putative transcription factors that are characterized by a carboxy-terminal leucine zipper and an adjacent TSC-box. This protein family is conserved from Caenorhabditis elegans to humans and is encoded by four separate loci in mammals, TSC22D1 to TSC22D4. These loci produce several isoforms that can be subdivided into a short and a long class depending on the length of the isoform-specific amino-terminal sequences and depending on the presence of two conserved, as-yet-uncharacterized motifs in the amino-terminal part of the long isoforms [12, 13]. In addition to the (partial) redundancy, synergistic and/or antagonistic functions among TSC-22 (TSC22D1.2) and its homologs are likely as TSC22DF proteins can form heterodimers  and may compete for common binding partners or target genes.
The short class of TSC22DF variants, including TSC-22 (TSC22D1.2), is well studied. In mice, TSC22D2 produces several short transcripts that are important for the osmotic stress response of cultured murine kidney cells . TSC22D3v2, also known as Gilz (glucocorticoid-induced leucine zipper), is required in the immune system for T-cell receptor mediated cell death [15–18]. Moreover, Gilz is a direct target gene of the transcription factor FoxO3 , and several binding partners of the Gilz protein are known, including NF-κB, c-Jun, c-Fos and Raf-1 [20–22]. In addition, short isoforms encoded by TSC22D3 have differential functions in the aldosterone response, sodium homeostasis and proliferation of kidney cells .
The function of long TSC22DF members is less well understood. The long isoform TSC22D1.1, produced by the TSC-22 locus, as well as the long human TSC22D2 protein are largely uncharacterized. TSC22D4 is important for pituitary development  and can form heterodimers with TSC-22 (TSC22D1.2) . Functional in vivo studies on TSC22DF, especially on the long isoforms, are needed to clarify how TSC-22 (TSC22D1.2) can act as a tumor suppressor.
Drosophila melanogaster is a valuable model organism for investigating the function of TSC22DF proteins in growth regulation for two reasons. First, many tumor suppressor genes  and growth-regulating pathways [26, 27] have been successfully studied in the fly. Second, the Drosophila genome contains a single locus, bunched (bun), encoding three nearly identical long and five short isoforms of TSC22DF members (FlyBase annotation FB2009_05 ). Thus, the redundancy and complexity of interactions among TSC22DF proteins are markedly lower in Drosophila than in mammals. Drosophila bun is important for oogenesis, eye development and the proper formation of the embryonic peripheral nervous system [29–31]. Furthermore, bun is required for the development of α/β neurons of the mushroom body, a brain structure involved in learning and memory . It has been proposed that bun acts as a mitotic factor during the development of α/β neurons.
Two studies that we and others carried out [12, 33] have demonstrated that, in addition to its role in patterning processes, bun plays a crucial role in growth regulation. Whereas the long Bun isoforms are positive growth regulators, genetic disruption of the short transcripts bunB-E and bunH does not alter growth. However, overexpression of bunB and bunC does interfere in a dominant-negative manner with normal bunA function. These results on Drosophila bun apparently contradict data describing mammalian TSC-22 as a growth-suppressing gene. To resolve this conflict, we hypothe-sized that the as-yet-uncharacterized long TSC-22 isoform (TSC22D1.1) is a functional homolog of BunA in growth regulation and that it is antagonized by the short isoform TSC22D1.2.
Here we investigate the evolutionary functional conservation between BunA and the human TSC22DF proteins. We report that long TSC-22 (TSC22D1.1) as well as the long human isoforms TSC22D2 and TSC22D4 can substitute for BunA function but the short isoforms cannot. In addition, we demonstrate that the growth-promoting function of BunA is - at least in part - mediated by Mlf1 adapter molecule (Madm). We have identified Madm in a genetic screen for growth regulators as well as in a proteomic screen for BunA-interacting proteins, and we show that BunA and Madm cooperate in promoting growth during development.
How BunA exerts its growth-regulating function is unknown. It is conceivable that a protein specifically binding to long TSC22DF isoforms accounts for the growth-promoting ability. Therefore, we set out to identify binding partners by means of pulldown experiments combining affinity purification and mass spectrometry (AP-MS) [36, 37]. As baits, we expressed green fluorescent protein (GFP)- or hemagglutinin (HA)-tagged versions of the full-length BunA protein (rather than BunA-specific peptides, which might not preserve the three-dimensional structure of BunA) in Drosophila S2 cells and affinity purified the protein complexes by means of anti-GFP or anti-HA beads, respectively. The purified complexes were analyzed by tandem mass spectrometry (LC-MS/MS), and the proteins identified were judged as good candidates if they satisfied the following three criteria: they were not found in control experiments (HA-tagged GFP was used as bait and affinity purified using anti-GFP or anti-HA beads); they showed up in several independent AP-MS experiments; and they had an identification probability above an arbitrary threshold (Mascot score 50). We identified the adapter protein Madm as a good candidate in two independent experiments [see Additional file 1].
Assuming that BunA and Madm interact, they should at least partially co-localize. Immunofluorescence studies in S2 cells revealed that GFP-BunA and HA-Madm signals in fact largely overlapped (Figure 2b, c). Interestingly, the HA-Madm signal was less dispersed when GFP-BunA was expressed in the same cell, indicating that the interaction with BunA altered the subcellular localization of HA-Madm (Figure 2c). A statistical analysis (Materials and methods) revealed that HA-Madm was only localized in punctae when co-overexpressed with GFP-BunA (100%, n = 50) but not when co-overexpressed with GFP (0%, n = 50). Moreover, when a mutated HA-Madm protein (R525H, see below) was expressed, the localization in punctae was lost in 66% of cells co-overexpressing GFP-BunA (n = 50). The GFP-BunA signal largely overlapped with the Golgi marker GMAP210  but not with an endoplasmic reticulum (ER) marker (Figure 2d, and data not shown), indicating that GFP-BunA localizes to the Golgi. The localization of BunA and Madm was not dependent on their tag because GFP- and HA-tagged BunA and Madm behaved similarly (data not shown). Furthermore, GFP-tagged BunA and Madm proteins were functional because they rescued the lethality of bun and Madm mutants, respectively, when expressed in the fly (Materials and methods). Taken together, our AP-MS and co-localization studies demonstrate that the adapter molecule Madm associates with BunA.
To investigate whether Madm binds to long-isoform-specific sequences, we mapped the Madm-binding region in BunA, and vice versa, by means of co-immunoprecipitation (co-IP) and yeast two-hybrid (Y2H) experiments. The advantage of the Y2H system is that Drosophila bait proteins are unlikely to form complexes or dimers - in case of BunA via its leucine zipper - with endogenous yeast proteins and therefore the observed Y2H interactions are presumably direct. Our co-IP and Y2H data indicated that a long-isoform-specific amino-terminal sequence of BunA (amino acids 475-553) encompassing motif 2 is sufficient for the interaction with Madm (Figure 2e and Additional file 2). Moreover, one of the two point mutations isolated in a genetic screen that affect motif 2 (the hypomorphic bun alleles A-R508W and A-P519L; see Additional data file 4 and ) weakened the binding to Madm.
In a parallel genetic screen based on the eyFLP/FRT recombinase system, we were searching for mutations that cause growth phenotypes akin to the bunA phenotype . A complementation group consisting of seven recessive lethal mutations was mapped to the Madm genomic locus (Materials and methods). The seven ethyl methanesulfonate (EMS)-induced mutations caused a small head (pinhead) phenotype; therefore, the affected gene encodes a positive growth regulator (Figure 3b, c). The rather compact genomic locus of Madm contains two exons and produces a single protein isoform (Figure 3e). The adapter protein Madm possesses a kinase-like domain that lacks the conserved ATP-binding motif, thus rendering it a non-functional kinase [39, 40]. Moreover, Drosophila Madm carries several conserved NESs and a non-conserved nuclear localization signal (NLS; Figure 3e) . We identified molecular lesions in all seven EMS-induced mutations (six point mutations and one deletion; Figure 3e) by sequencing the Madm open reading frame (ORF). Expression of a genomic Madm as well as of a UAS-Madm construct was sufficient to rescue the lethality of the seven alleles and one copy of the genomic Madm construct fully reverted the pinhead phenotype (Materials and methods; Figure 3d), proving that Madm mutations caused the growth deficit.
To characterize the Madm growth phenotype more closely, we first attempted to order the Madm alleles according to their strength. To determine the lethal phase of the recessive lethal Madm EMS-alleles, they were combined with a deficiency (Df(3R)Exel7283) uncovering the Madm locus (see also Materials and methods). Development of mutant larvae ceased mostly in the third larval instar and in the prepupal stage. The onset of the prepupal stage was delayed by 2 to 10 days. Alleles 2D2, 2U3, and 3G5 led to strong growth deficits, most apparent in L3 larvae, whereas alleles 3Y2, 4S3, and 7L2 caused almost no reduction in larval size. The allele 3T4 turned out to be a hypomorphic allele capable of producing few adult flies (less than 10% of the expected Mendelian ratio). 3T4 is caused by a point mutation leading to a premature translational stop (Figure 3e). However, it has been reported that the translation machinery can use alternative start codons in human Madm that are located further downstream . Alternative start codons are also present in Drosophila Madm and may account for the hypomorphic nature of the allele 3T4.
As a second measurement of the strength of the Madm alleles, the severity of the pinhead phenotypes was judged. Consistent with the first assay, alleles 2D2, 2U3, and 3G5 produced the most severe pinhead phenotypes (Figure 3c); alleles 3Y2, 4S3, and 7L2 displayed pinhead phenotypes of intermediate strength (Figure 3b); and allele 3T4 led to a very mild reduction in head and eye size in the eyFLP/FRT assay (data not shown).
Furthermore, the body size of rare hypomorphic mutant flies (produced with allele 3T4) was reduced (Figure 4f), and females were almost 40% lighter than controls (Figure 4g). Madm escapers also displayed malformations such as eye and wing defects. Eye sections revealed rotation defects, missing and extra photoreceptors, fused ommatidia, and cell-fate transformations (Figure 4h, and data not shown). Similar patterning defects were observed in Madm mutant clones in the eye (Figure 4b', c'). The wing phenotypes ranged from no defects to wing notches and an incomplete wing vein V (Figure 4i). All the growth and patterning defects of Madm mutant viable flies were reverted by a genomic rescue construct (Figure 4f, g; data not shown).
Thus, Madm controls cell number and cell size and also controls patterning processes in the eye and the wing. These phenotypes strongly resemble phenotypes displayed by bunA mutant cells and flies  [see Additional file 5 for wing notches], although the pinhead phenotype and the eye-patterning defects caused by the strong Madm alleles 2D2 and 3G5 are more severe.
In the present study, we provide genetic evidence for an evolutionarily conserved function of the long TSC22DF isoforms in the control of cell and organ size. Because the long TSC22DF proteins share two conserved motifs in their amino-terminal parts, we set out to identify specific binding partners that cooperate with the long isoforms to promote cellular growth. The combination of AP-MS experiments with a genetic screen for novel mutations affecting growth  resulted in the identification of Madm as a strong candidate for such an interactor, illustrating the synergistic forces of the two approaches.
We found that all long - but none of the short - members of the human TSC22DF are able to replace the function of BunA in the fly. Thus, the potential of long isoforms to positively regulate growth has been conserved through evolution. Conceivably, the various long isoforms present in mammals can, at least to some extent, substitute for one another and hence act in a (partially) redundant manner. However, our rescue experiments in Drosophila only demonstrate the potential of the long human TSC22DF proteins and do not allow us to draw any conclusions about their endogenous function. Whether TSC22D1.1 is indeed a functional homolog of BunA in growth regulation and whether the short TSC22D1.2 protein antagonizes it need to be addressed in mammalian in vivo systems.
The potential of long human TSC22DF proteins to replace BunA function is likely to reside in conserved sequences shared by all long TSC22DF members. Alignments with long TSC22DF proteins revealed two short stretches of high conservation [12, 13]. Intriguingly, two EMS-induced mutations leading to amino acid substitutions in the second conserved motif were isolated in a genetic screen for mutations affecting growth .
The corresponding alleles behaved as strong bunA hypomorphs that were recessive lethal and caused severe growth deficits. BunA binds via the second conserved motif to Madm and at least one mutation weakens the binding but does not abolish it. As the motif 2 is present in all long TSC22DF isoforms, it is likely that all of them can bind Madm. In fact, the long human isoform TSC22D4 is able to do so, as uncovered in a large-scale Y2H study [42, 43]. So far, we could not assign any function to the first conserved motif. Because this motif is heavily phosphorylated , we speculate that it is important for the regulation of BunA activity.
Because short isoforms can heterodimerize with long isoforms, as reported for TSC-22 (TSC22D1.2) and TSC22D4 , they may interact indirectly with Madm. This could explain why human Madm was found to interact with the bait protein TSC-22 (TSC22D1.2) in a high-throughput analysis of protein-protein interactions by immunoprecipitation followed by mass spectrometry (IP/MS) [43, 45]. Moreover, we found that the short isoform BunB interacts with Drosophila Madm in a co-IP but not in a Y2H assay. Heterodimers of BunA and short Bun isoforms exist in Drosophila S2 cells because we found that a small fraction of endogenous BunA did co-immunoprecipitate with tagged BunB and BunC versions (data not shown). However, we failed to identify short Bun isoforms as BunA heterodimerization partners in the AP-MS experiments. One possible explanation is that the peptides specific for short Bun isoforms are very low abundant. This might also explain why they were not detected when a catalog of the Drosophila proteome was generated .
In mammalian cells, both IP/MS and Y2H experiments provided evidence for a physical interaction between Madm and TSC22DF proteins [42, 43]. Our study extends these findings in two ways. We demonstrate that only long TSC22DF proteins directly bind to Madm, and we also provide evidence for the biological significance of this interaction in growth control.
Madm has been implicated in ER-to-Golgi trafficking because overexpression of Madm affected the intracellular transport of a Golgi-associated marker in COS-1 cells . In addition, Madm localizes to the nucleus, the cytoplasm and Golgi membranes in Drosophila, and an RNA interference (RNAi)-mediated knockdown of Madm in cultured cells interfered with constitutive protein secretion [46, 48]. In Xenopus, Madm is important for eye development and differentiation . Thus, it is apparent that Madm is involved in biological processes other than growth control. As a consequence, disruption of Madm leads to complex phenotypes partly different from bunA phenotypes, and concomitant loss of Madm and bunA causes an even stronger growth decrease than the single mutants [see Additional file 5]. In addition to the Madm growth phenotypes, we observed patterning defects, for example in the adult fly eye and wing. Similar phenotypes were detected when bunA function was absent or diminished , yet the patterning defects caused by Madm and the Madm pinhead phenotype appeared to be more pronounced. Alternatively, these more pronounced phenotypes could arise from a lower protein stability of Madm compared with BunA, leading to more severe phenotypes in the eyFLP/FRT assay. However, in contrast to the effects of BunA overexpression, the overexpression of Madm early during eye and wing development led to severe differentiation defects. These phenotypes could be caused by Madm-interaction partners other than BunA that function in different biological processes.
Madm is an adapter molecule that has several interaction partners in mammals. Originally, it was proposed that Madm - also named nuclear receptor binding protein 1 (NRBP1) in humans - binds to nuclear receptors because of the presence of two putative nuclear-receptor-binding motifs . However, Madm has never been experimentally shown to bind to any nuclear receptor. Furthermore, the nuclear-receptor-binding motifs are not conserved in Drosophila. From studies in mammalian cells, it is known that Madm can bind to murine Mlf1 , Jab1 (Jun activation domain-binding protein 1) , activated Rac3 (Ras-related C3 botulinum toxin substrate 3) , Elongin B , and the host cellular protein NS3 of dengue virus type 2 . Indeed, in our AP-MS experiment where HA-Madm was used as bait, we identified Elongin B but not Mlf1 (dMlf in Drosophila), Jab1 (CSN5 in Drosophila) or Rac3 (RhoL in Drosophila). It is possible that these interactions are not very prominent or even absent in Drosophila S2 cells.
Madm and BunA are limiting components of a newly identified growth-promoting complex because genetic disruptions of bunA and Madm both result in a reduction in cell number and cell size. However, to enhance the activity of the complex and thereby to augment organ growth, simultaneous overexpression of both components is required. In the reduction-of-function situation, we did not detect genetic interactions between bunA and Madm. Thus, we hypothesize that both proteins are essential components of a growth-promoting complex. As a consequence, the phenotype of the limiting protein will be displayed no matter whether the levels of the other protein are normal or lowered.
It is not clear whether additional proteins are part of the Madm-BunA growth-regulating complex. Heterodimerization partners of BunA or other Madm-binding proteins are candidate complex members. Conversely, Madm-binding partners could form distinct complexes mediating different functions. These complexes may negatively regulate each other by competing for their shared interaction partner Madm. Indeed, we observed a suppressive effect when dMlf or CSN5 were co-overexpressed along with Madm and BunA in the developing eye (data not shown). Thus, other Madm-binding partners will directly or indirectly influence the growth-promoting function of the Madm-BunA complex.
We found that GFP-BunA co-localizes with the Golgi marker GMAP210 in Drosophila S2 cells. Interestingly, it has been suggested that mammalian as well as Drosophila Madm plays a role in ER-to-Golgi transport, and it has been reported that Madm localizes to the cytoplasm, weakly to the nucleus, and to the Golgi in Drosophila S2 cells . We observed a similar subcellular localization of both HA-Madm and HA-Madm(R525H) when expressed at low levels (data not shown). The Golgi localization was lost in cells expressing higher levels of HA-Madm, possibly because the cytoplasm was loaded with protein. Intriguingly, the Golgi localization of HA-Madm, but not of HA-Madm(R525H), was completely restored in cells coexpressing GFP-BunA and HA-Madm at relatively high levels. Thus, BunA is able to direct Madm to the Golgi, and the Golgi may be the site of action of the Madm-BunA growth-regulating complex. However, because our investigation was restricted to overexpression studies, the subcellular localization of endogenous Madm and BunA remains to be analyzed.
How could binding of Madm modulate the function of BunA? Madm could have an impact on the stability, the activity or the subcellular localization of BunA. We analyzed the amount of endogenous and overexpressed BunA protein in cultured Drosophila cells with diminished or elevated Madm levels, produced by RNAi with double-stranded RNA (dsRNA) or by overexpression, respectively, but did not observe any effect (data not shown). Thus, Madm does not fundamentally affect the stability of BunA. The putative transcription factor BunA localizes to the cytoplasmic and not to the nuclear fractions in Drosophila [31, 46]. Because Madm possesses NES and NLS sequences, it is likely to shuttle between the cytoplasm and the nucleus  and it might therefore transport BunA to the nucleus, where BunA could act as a transcription factor. So far, however, we have not detected nuclear translocation of BunA (data not shown). The activity of BunA could be controlled by phosphorylation events, as it has been described for numerous transcription factors. An attractive model is that a kinase binding to Madm phosphorylates BunA. An analogous model was proposed for murine Mlf1 as Madm binds to an unknown kinase that phosphorylates Madm itself and a 14-3-3zeta-binding site in Mlf1, possibly resulting in 14-3-3-mediated sequestration of Mlf1 in the cytoplasm .
Further studies will be required to solve the exact mechanism by which Madm and BunA team up to control growth. We anticipate that our findings will encourage studies in mammalian systems on the function of long TSC22DF members, in particular TSC22D1.1, in growth control.
The mechanism by which the tumor suppressor TSC-22 acts has remained unclear, and the functional analysis of TSC-22 is hampered because of redundancy and various possible interactions among the homologous TSC22DF proteins. In a previous study, we showed that the Drosophila long class TSC22DF isoforms are positive growth regulators. Here, we report that the long human TSC22DF isoforms are able to substitute for BunA function when expressed in the fly. To illuminate the mechanism by which long TSC22DF isoforms promote growth, we searched for BunA binding partners. A combined proteomic and genetic analysis identified the adapter protein Madm. Drosophila Madm is a positive growth regulator that increases organ growth when co-overexpressed with BunA. We propose that the BunA-Madm growth-promoting complex is functionally conserved from flies to humans.
Flies were kept at 25°C on food described in . For the rescue experiment bun 200B , UAS-bunA , arm-Gal4, da-Gal4, and Act5C-Gal4 (Bloomington Drosophila Stock Center), and vas-ϕC31-zh2A; ZH-attP-86Fb  flies were used. For the genetic mosaic screen, y, w, eyFLP; FRT82B, w +, cl 3R3 /TM6B, Tb, Hu flies  were used. Clonal analyses in adult eyes were carried out with y, w, hsFLP; FRT82B, w +, M/TM6B, Tb, Hu, y +. For rescue experiments, allelic series, and the analysis of hypomorphic mutant Madm flies, Df(3R)Exel7283 (Bloomington Drosophila Stock Center) was used. In hypomorphic bunA flies displaying wing notches, the alleles bun A-P519L  and bun rI043  were combined. Madm, bunA double-mutant mosaic heads were generated with y, w, eyFLP; FRT40A, w +, cl 2L3 /CyO; FRT82B, w +, cl 3R3 /TM6B, Tb, Hu  flies, bun allele A-Q578X , the UAS hairpin line 19679 (RNAi bun) , and ey-Gal4 . The overexpression studies in the eye and wing were done with GMR-Gal4  and C10-Gal4 , UAS-eGFP, and UAS-lacZ (Bloomington Drosophila Stock Center).
bunA cDNA was subcloned from a UAS-bunA plasmid  into the pUAST-attB vector  using EcoRI sites. The bunA ORF was PCR-amplified from a UAS-bunA plasmid , cloned into the pENTR-D/TOPO vector (Invitrogen) and subcloned into a Gateway-compatible pUAST-attB vector (J Bischof, Institute of Molecular Biology, University of Zurich; unpublished work) by clonase reaction (LR clonase II enzyme).
The human ORFs TSC22D1.1, TSC22D1.2, TSC22D3v1-3 and TSC22D4 were derived from the cDNA of a normal prostate tissue sample. This sample was derived from a radical prostatectomy specimen at the Department of Urology, University of Berne as described previously . The ORF TSC22D2 was derived from the pOTB7 vector carrying the TSC22D2 full-length cDNA (Open Biosystems, clone ID 5454441). ORFs were PCR-amplified, cloned into the pGEM-T Easy vector (Promega) and subsequently cloned into the pcDNA3.1/Hygro(+) vector (Invitrogen). The ORFs TSC22D1.1 and TSC22D2 were subcloned from pGEM-T Easy to pUAST-attB using EcoRI. The ORF TSC22D1.2 was subcloned from pcDNA3.1/Hygro(+) to the pBluescript II KS(+/-) vector using HindIII and XhoI, then further subcloned into the pUAST vector  using EcoRI and XhoI, and finally cloned into the pUAST-attB vector with EcoRI and XbaI. The ORFs TSC22D3v1-3 and TSC22D4 were PCR-amplified from cDNA-containing pGEM-T Easy plasmids and cloned into pUAST-attB using EcoRI and NotI (restriction sites added by PCR). The pUAST-attB plasmids were injected into vas-ϕC31-zh2A; ZH-attP-86Fb embryos .
Madm cDNA was cleaved by EcoRI and HindIII double digestion from expressed sequence tag (EST) clone LD28567 (Berkeley Drosophila Genome Project) and subcloned into pUAST using the same restriction sites to generate the UAS-Madm construct. Madm genomic DNA (from 559 bp upstream of Madm exon 1 (containing exon 1 of the neighboring gene CG2097) to 1,681 bp downstream of Madm exon 2) was amplified by PCR using forward primer GCTCTAGAAGGCGATGCGATGACCAGCTC and reverse primer GAGATCTTC-ATGACGTTTTCCGCGCACTCGAGT. The PCR product was digested with BglII and XbaI and subcloned into the transformation vector pCaspeR.
The complete and partial ORFs of bunA and Madm were PCR-amplified from a pUAST-bunA  and a UAS-Madm plasmid, respectively, and cloned into the pENTR/D-TOPO vector. The point mutations in pENTR-D/TOPO-bunA and -Madm were introduced by substitution of a BamHI/DraI and an FspI/SacI fragment that was PCR-amplified using mutated primers. By clonase reaction (LR clonase II) the inserts were transferred to the following destination vectors: pMT-HHW-Blast (O Rinner, IMSB, ETH Zurich, unpublished work), pMT-GW-Blast, pDEST22, and pDEST32. Additionally, the GFP ORF was cloned into the pMT-HHW-Blast vector, leading to the production of HA-tagged GFP as a negative control for co-IP experiments. The pMT-HHW-Blast vector is based on the pMT-V5HisA vector (Invitrogen) carrying a metallothionein-inducible promoter. The multiple cloning site and tag sequences were replaced by the Gateway cassette, including the coding sequence for a triple HA-tag from the pAHW destination vector (Invitrogen). The blasticidin-resistance cassette was cloned from the pCoBlast vector (Invitrogen) into the pMT-V5HisA vector backbone. The pMT-HHW-Blast vector was modified by exchanging an AgeI/EcoRI fragment containing the GFP coding region derived from the pAGW destination vector.
Drosophila embryonic S2 cells were grown at 25°C in Schneider's Drosophila medium (Gibco/Invitrogen) supplemented with 10% heat-inactivated fetal calf serum (FCS), as well as penicillin and streptomycin. S2 cells were transfected according to the Effectene transfection protocol for adherent cells (Qiagen). To generate stable cell lines, transfected S2 cells were selected for 14-30 days in Schneider's medium containing 25 μg/ml blasticidin and afterwards propagated in Schneider's medium containing 10 μg/ml blasticidin.
Before affinity purification, Drosophila S2 cells were grown in shaking flasks. Bait expression was induced by 600 μM CuSO4 for at least 16 h. For affinity purification the cell pellets were lysed on ice for 30 minutes in 10 ml HNN (50 mM HEPES pH 7.5, 5 mM EDTA, 250 mM NaCl, 0.5% NP40, 1 mM PMSF, 50 mM NaF, 1.5 mM Na3VO4, protease inhibitor cocktail (Roche)) in the presence of 3 mM dithiobis-(succinimidyl propionate) (DSP) with ten strokes using a tight-fitting Dounce homogenizer. Reactive DSP was quenched by adding 1 ml Tris pH 7.5. Insoluble material was removed by centrifugation and the supernatant was precleared using 100 μl Protein A-Sepharose (Sigma) for 1 h at 4°C on a rotating shaker. After removal of the Protein A-Sepharose, 100 μl Agarose anti-GFP beads (MB-0732) or Agarose monoclonal mouse anti-HA beads (Sigma A2095) were added to the extracts and incubated for 4 h at 4°C on a rotating shaker. Immunoprecipitates were washed four times with 20 bed volumes of lysis buffer and three times with 20 bed volumes of buffer without detergent and protease inhibitor. The proteins were released from the beads by adding three times 150 μl 0.2 M glycine pH 2.5. Following neutralization with 100 μl 1 M NH4CO3, the eluates were treated with 5 mM tris(2-carboxyethyl)phosphine (TCEP) to reduce S-S bonds and DSP crosslinkers for 30 minutes at 37°C, and alkylated with 10 mM iodoacetamide for 30 minutes at room temperature in the dark. For tryptic digestion, 1 μg trypsin was added to the eluate and incubated at 37°C overnight.
Nanoflow-LC-MS/MS was performed by coupling an UltiMate HPLC system (LC-Packings/Dionex) in-line with a Probot (LC-Packings/Dionex) autosampler system and an LTQ ion trap (Thermo Electron). Samples were automatically injected into a 10-μl sample-loop and loaded onto an analytical column (9 cm × 75 μm; packed with Magic C18 AQ beads 5 μm, 100 Å (Michrom BioResources)). Peptide mixtures were delivered to the analytical column at a flow rate of 300 nl/minute of buffer A (5% acetonitrile, 0.2% formic acid) for 25 minutes and then eluted using a gradient of acetonitrile (10-45%; 0.5%/minutes) in 0.2% formic acid. Peptide ions were detected in a survey scan from 400 to 2,000 atomic mass units (amu; one to two μscans) followed by three to six data-dependent MS/MS scans (three μscans each, isolation width 2 amu, dynamic exclusion list 250, dynamic exclusion time 240 sec, two repeats) in an automated fashion. Following analysis, raw MS/MS data were converted to Mascot generic format (MGF) files that were used to identify the corresponding peptides using the Mascot database search tool (MatrixScience) [59, 60]. MS/MS spectra were searched against the Drosophila protein database (dmel_r5.18_FB2009_05 released 20090529)  with the following criteria: requirement for trypsin digestion; peptide mass tolerance 2 Da; fragment mass tolerance 0.6 Da; missed cleavage for trypsin 3; fixed modification carbamidomethyl (C); variable modifications acetyl (N-term), oxidation (M), CAM-thiopropanoyl (K) (derived from DSP crosslinker). All peptide assignments with Mascot ion score larger than the homology score and with Mascot expect score smaller than 0.05 (significant ion score) were considered as good hits.
For immunofluorescence Drosophila S2 cells were stimulated for 4 h with 600 μM CuSO4 and spread on concanavalin-A-treated slides and fixed with 4% paraformaldehyde. Mouse anti-HA (1:200, Roche 166606), rabbit anti-GMAP210 (1:200) , goat anti-mouse Cy3 (1:200, Amersham PA43002) and goat anti-rabbit Cy3 (1:200, Amersham PA43004) antibodies were used. Nuclei were visualized by DAPI (100 ng/ml) staining. For imaging, a Leica TCS SPE confocal microscope was used.
Statistical analysis of the dependence of HA-Madm localization on GFP-BunA was carried out in S2 cells transiently transfected two days before analysis. Cells were co-transfected with pMT-HA-Madm or pMT-HA-Madm(R525H) and with either empty pMT-GW-Blast (for control GFP expression) or with pMT-GFP-bunA. Fifty cells were analyzed for each combination. The expressed HA-Madm and HA-Madm(R525H) proteins showed a similar diffuse localization in the cytoplasm of cells strongly expressing GFP (50 out of 50 each). By contrast, HA-Madm localized to dots (punctae) in cells displaying a readily detectable GFP-BunA signal (50 out of 50). In 17 out of 50 cells, GFP-BunA directed HA-Madm(R525H) localization in punctae.
To generate flies expressing amino-terminally GFP-tagged versions of BunA and Madm, the respective ORFs were subcloned by clonase reaction from pENTR/D-TOPO to pUAST-GW-AttB (the Gateway-compatible pUAST-AttB vector was provided by I Pörnbacher, IMSB, ETH Zurich; unpublished work). The plasmid containing bunA was injected into vas-ϕC31-zh2A; ZH-attP-86Fb embryos , and the Madm-containing plasmid into vas-ϕC31-zh2A; ZH-attP-51D embryos . Leaky expression of UAS-GFP-bunA was sufficient to completely rescue the lethality of bun 200B/200B mutants. Expression of UAS-GFP-Madm under the control of the arm-Gal4 driver line resulted in a rescue (approximately 50% of the expected Mendelian ratio) of the lethality of Madm 3Y2/Df(3R)Exel7283 animals.
Stable Drosophila S2 cell lines capable of producing GFP (negative control) or GFP-tagged Bun versions were transiently transfected with HA-Madm plasmids. Two days after transient transfection, confluent Drosophila S2 cells (2.3 ml corresponding to one well of a 6-well-plate) were induced for 4 h with CuSO4 (600 μM), harvested, and washed with PBS. Cells were lysed in IP buffer (120 mM NaCl, 50 mM Tris pH 7.5, 20 mM NaF, 1 mM benzamidine, 1 mM EDTA, 6 mM EGTA, 15 mM Na4P2O7, 0.5% Nonidet P-40, 1× Complete Mini Protease Inihibitor (Roche)). After incubation for 15 minutes on an orbital shaker at 4°C, solubilized material was recovered by centrifugation at 13,000 rpm for 15 minutes and supernatants were collected. Cell lysates were incubated for 4 h at 4°C under rotation either with 20 μl Agarose anti-GFP beads (MB-0732) or Agarose monoclonal mouse anti-HA beads (Sigma A2095) that had been equilibrated with IP buffer. Beads were then washed five times with IP buffer and boiled for 5 minutes at 95°C in Laemmli buffer. Proteins contained in the supernatant were separated by SDS-PAGE. For western blotting, the Hybond ECL Nitrocellulose membrane (Amersham), the ECL detection reagent (Amersham), and the following antibodies were used: rabbit anti-Bun (1:1,000) , rabbit anti-BunA (1:2,000), mouse anti-HA (1:3,000, Roche 166606), monoclonal mouse anti-GFP (1:1,000, Roche 11 814 460 001), monoclonal mouse anti-rabbit horseradish peroxidase (HRP) (1:10,000, Jackson Lab), sheep anti-mouse HRP (1:10,000, Amersham NA931).
The rabbit anti-BunA antibody was generated using the following peptide to immunize rabbits: H2N-TNRKPKTTSSFEC-CONH2 (Eurogentec). The serum was double-affinity purified against the peptide coupled to a column. Specificity of the antibody was shown by western blotting: Drosophila S2 cells were incubated for 2 days with dsRNA  that targets either the ORF of bunA (500 bp long dsRNA) or of GFP as a control (700 bp long dsRNA). Primer sequences are available on request.
For the Y2H experiments the Gateway-compatible ProQuest Two-Hybrid System (Invitrogen) including the pDEST32 and pDEST22 vectors was used. Transformation of a MaV203 strain was achieved with the LiAc/SS carrier DNA/polyethylene glycol (PEG) method. To identify interactions, yeast cells were tested for HIS3 reporter gene expression under the control of the HIS promoter. The competitive inhibitor 3-amino-1,2,4-triazole (3-AT) was used to dampen leaky expression. The 3-AT concentration needed to restrain leakiness was determined to be 10 mM by almost suppressing the growth of negative control strains that have been transformed with an empty pDEST22 and/or pDEST32 vector (every combination of negative controls was examined). For each interaction to be tested, five yeast colonies were pooled and grown overnight in -Leu -Trp medium. Seven microliters of dilutions of OD600 = 0.1, 0.01, and 0.001 with double-distilled H2O were spotted on -Leu -Trp -His +3-AT (10 mM) plates and incubated for 52-56 h at 30°C. As a control for a correct dilution series they were also spotted on -Leu -Trp -His plates without 3-AT (data not shown).
The eyFLP/FRT technique  was used to produce mosaic flies with eyes and head capsules largely homozygous for randomly induced mutations. The rest of the body (including the germline) remained heterozygous and was therefore phenotypically wild type (screen described in ). The seven EMS alleles of a complementation group on 3R were mapped using visible markers (P-elements) to the cytological region 83-84. With deletions that failed to complement the lethality of EMS alleles (Df(3R)ED5196, Df(3R)ED5197, Df(3R)Exel7283, and Df(3R)Exel6145) the candidate region was narrowed down to the cytological interval 83C1-4. The EP-element EP3137 inserted in the 5' untranslated region of the Madm locus failed to complement the lethality of the EMS alleles.
The UAS/Gal4 system  was used to test whether ubiquitous expression of a UAS-Madm construct during development - achieved by the arm-Gal4, da-Gal4, and Act5C-Gal4 driver lines - rescued the recessive lethality of the EMS alleles. Using arm-Gal4, the viability of combinations of EMS alleles (2U3, 3G5, 3Y2, and 7L2) with the deletion Df(3R)Exel7283 was completely restored and the lethality of heteroallelic combinations among EMS alleles was partially rescued. One copy of genomic Madm rescue construct (LCQ139) - comprising 559 bp of the upstream region, the two Madm exons and the intron, and 1,681 bp of downstream sequences - was sufficient to entirely rescue the lethality of heteroallelic combinations of EMS alleles (2U3 and 3G5) and of the hemizygous alleles (tested with the deficiency Df(3R)Exel7283). In addition, the pinhead phenotypes of the EMS alleles 2U3 and 3G5 were reverted by one copy of the genomic construct.
Animals were reared on apple agar plates supplemented with yeast at 25°C. Allelic series was determined by crossing Madm EMS alleles (y, w; FRT82B, Madm - /TM6B, Tb, Hu) to a deficiency (y, w; Df(3R)Exel7283/TM6B, Tb, Hu) uncovering the entire Madm locus. In addition, the development of Madm 2U3/3G5 and Madm 3Y2/7L2 animals was compared with the development of Madm 2U3 or 3G5 /Df(3R)Exel7283 and Madm 3Y2 or 7L2 /Df(3R)Exel7283 animals, respectively. Heteroallelic combinations of the Madm EMS alleles, except for 3T4, resulted in larval phenotypes that were as strong as the phenotypes caused in the hemizygous condition.
Clones in the adult eyes were induced 24-48 h after egg deposition (AED) by a heat shock for 1 h at 34°C in animals of the genotype y, w, hsFLP/y, w; FRT82B, w +, M/FRT82B, Madm -. Adult fly heads were halved using a razor blade and stored up to 1 h in Ringer's solution on ice. Eyes were then fixed and processed as described in . Pictures were taken with a Zeiss Axiophot microscope. In tangential eye sections, the areas enclosed by rhabdomeres and cell bodies from photoreceptors R1-R6 were measured in mutant ommatidia (lacking pigmentation) and in neighboring wild-type sized (pigmented) ommatidia using Adobe Photoshop. Student's t-test was used to determine significance.
For the analysis of the ommatidia number in mosaic eyes and the analysis of ommatidia size in overexpression studies, flies were frozen at -20°C before taking SEM pictures. All ommatidia were counted and the area of seven adjacent ommatidia (rosette) in the center was measured using Adobe Photoshop.
Freshly eclosed hypomorphic mutant Madm flies were kept on fresh food for 2 days. Flies were exposed to 95°C for 5 minutes and air-dried at room temperature for 3 days. The dry weight of individual flies was determined with a Mettler Toledo MX5 microbalance. Significance was assessed using Student's t-test.
Adult wings were mounted in Euparal after dehydration in 70% and subsequently 100% ethanol. Pictures were taken with a Zeiss Axiophot microscope. Significance was assessed using Student's t-test.
For the overexpression studies, a set of Gal4 driver lines was crossed to a UAS-Madm transgenic line. No obvious phenotypes were observed using arm-Gal4, da-Gal4, ppl-Gal4, and sev-Gal4. Ubiquitous overexpression achieved with Act5C-Gal4 resulted in lethality. Expression in the dorsal compartment of the developing wing (ap-Gal4) led to deformed wings. MS1096-Gal4 directed expression in the developing wing produced vein defects and blisters in the adult wing. Expression of Madm during early eye development (ey-Gal4) produced patterning defects (rough and small adult eyes) whereas Madm expression later during eye development (GMR-Gal4) produced growth phenotypes when co-overexpressed with UAS-bunA.
green fluorescent protein
Mlf1 adapter molecule
Mascot generic format
Myeloid leukemia factor 1
nuclear export signal
nuclear localization signal
Transforming growth factor-β1 stimulated clone-22
TSC-22 domain family
We thank Anni Straessle, Béla Brühlmann, Christof Hugentobler and Rita Bopp for technical assistance; Johannes Bischof, Oliver Rinner and Ingrid Pörnbacher for reagents; Fabian Rudolf and Daniel Bopp for help with the yeast two-hybrid experiments; Timo Glatter, Matthias Gstaiger, Cristian Köpfli and Sandra Götze for assistance in the AP-MS analysis; Marjorie Cote, Raphael Hafen, Sabina Wirth-Hafen and Désirée Haltiner for their contributions in an undergraduate course; and Peter Gallant, Christian Frei and Hafen lab members for helpful discussions. This work was supported by the Swiss National Science Foundation (SNF) and the ETH Zurich.
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