Browse Subject Areas

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

For more information about PLOS Subject Areas, click here.

  • Loading metrics

Transgenic Drosophila for Investigating DUX4 and FRG1, Two Genes Associated with Facioscapulohumeral Muscular Dystrophy (FSHD)

  • Takako I. Jones , (TIJ); (PLJ)

    Affiliations The Department of Cell and Developmental Biology, University of Massachusetts Medical School Worcester, Massachusetts, United States of America, The Department of Cell and Developmental Biology, University of Illinois at Urbana-Champaign, Urbana, Illinois, United States of America

  • Megan Parilla,

    Affiliation The Department of Cell and Developmental Biology, University of Illinois at Urbana-Champaign, Urbana, Illinois, United States of America

  • Peter L. Jones (TIJ); (PLJ)

    Affiliations The Department of Cell and Developmental Biology, University of Massachusetts Medical School Worcester, Massachusetts, United States of America, The Department of Cell and Developmental Biology, University of Illinois at Urbana-Champaign, Urbana, Illinois, United States of America

Transgenic Drosophila for Investigating DUX4 and FRG1, Two Genes Associated with Facioscapulohumeral Muscular Dystrophy (FSHD)

  • Takako I. Jones, 
  • Megan Parilla, 
  • Peter L. Jones


Facioscapulohumeral muscular dystrophy (FSHD) is typically an adult onset dominant myopathy. Epigenetic changes in the chromosome 4q35 region linked to both forms of FSHD lead to a relaxation of repression and increased somatic expression of DUX4-fl (DUX4-full length), the pathogenic alternative splicing isoform of the DUX4 gene. DUX4-fl encodes a transcription factor expressed in healthy testis and pluripotent stem cells; however, in FSHD, increased levels of DUX4-fl in myogenic cells lead to aberrant regulation of target genes. DUX4-fl has proven difficult to study in vivo; thus, little is known about its normal and pathogenic roles. The endogenous expression of DUX4-fl in FSHD-derived human muscle and myogenic cells is extremely low, exogenous expression of DUX4-fl in somatic cells rapidly induces cytotoxicity, and, due in part to the lack of conservation beyond primate lineages, viable animal models based on DUX4-fl have been difficult to generate. By contrast, the FRG1 (FSHD region gene 1), which is linked to FSHD, is evolutionarily conserved from invertebrates to humans, and has been studied in several model organisms. FRG1 expression is critical for the development of musculature and vasculature, and overexpression of FRG1 produces a myopathic phenotype, yet the normal and pathological functions of FRG1 are not well understood. Interestingly, DUX4 and FRG1 were recently linked when the latter was identified as a direct transcriptional target of DUX4-FL. To better understand the pathways affected in FSHD by DUX4-fl and FRG1, we generated transgenic lines of Drosophila expressing either gene under control of the UAS/GAL4 binary system. Utilizing these lines, we generated screenable phenotypes recapitulating certain known consequences of DUX4-fl or FRG1 overexpression. These transgenic Drosophila lines provide resources to dissect the pathways affected by DUX4-fl or FRG1 in a genetically tractable organism and may provide insight into both muscle development and pathogenic mechanisms in FSHD.


Facioscapulohumeral muscular dystrophy (FSHD), one of the most prevalent late onset myopathies [~5–12 clinically affected subjects per 100,000 [1, 2]], is characterized by progressive, often asymmetric, weakness and atrophy of specific muscle groups [35]. The onset of clinical presentation normally occurs in the second or third decade of life with the muscles of the face and upper body typically affected first, followed by muscles of the lower extremities [3, 4]; however, there is a great range in clinical severity between FSHD subjects. For example, in the severe infantile cases, clinical weakness is apparent from early childhood [68], while other carriers may remain asymptomatic throughout their lifetimes [3, 915]. Overall, individual FSHD patients exhibit wide variability in age of onset, disease progression, and clinical severity, suggestive of genetic or epigenetic modifiers of the pathogenic pathway [3, 4, 7, 9, 10, 1417].

There are two genetic classes of FSHD (FSHD1, OMIM 158900; FSHD2, OMIM 158901) that share a common pathogenic mechanism linked to epigenetic changes in the chromosome 4q35 D4Z4 macrosatellite array and subtelomeric region [1719]. This strong epigenetic component of FSHD may account for much of the incomplete penetrance and high clinical variability in the disease presentation [1517, 20, 21]. Epigenetic derepression of the 4q35 D4Z4 region leads to the aberrant increased expression of the pathogenic isoform of the DUX4 gene encoded within the 4q35 D4Z4 array (Fig 1A) [16, 17, 19, 2224]. Thus, FSHD is essentially a dominant gain-of-function disease, which makes it amenable to being recapitulated, at least in part, by transgenic overexpression in model organisms.

Fig 1. The DUX4 model of FSHD.

(A) A model of the human system, which represents a summary of published work relevant to understanding FRG1 and DUX4 in relation to FSHD supplied to aid the reader with context, showing the FSHD-associated human chromosome 4q35 D4Z4 macrosatellite in healthy (upper) and FSHD (lower) subjects. In healthy subjects, the D4Z4 array consists of between 11 and ~120 D4Z4 repeat units (RU) and is epigenetically repressed (black lollipops). FRG1 is ubiquitously expressed, but there is no (or very little) polyadenylated DUX4-fl mRNA expression. In FSHD1 subjects, the D4Z4 array consists of between 1 and 10 D4Z4 RU, is epigenetically derepressed (yellow lollipops), and a significantly higher fraction of cells than in healthy subjects express polyadenlylated DUX4-fl mRNA. The DUX4-FL protein, a transcription factor that regulates many genes, can bind to an enhancer located in intron 2 of FRG1, and expression levels of FRG1 are moderately increased in these DUX4-FL expressing cells [34]. (B) The polyadenylated DUX4-fl mRNA is derived from the distal repeat of the D4Z4 array. There are two potential translation start sites for DUX4-fl, termed MKG and MAL. Transgenic Drosophila UAS-DUX4-flMKG and UAS-DUX4-flMAL contain the coding sequence, codon optimized for Drosophila, from the indicated start codon through the stop codon (red *) in exon 1. Please see the following reviews for relevant references relating to FSHD depicted in this figure [17, 21, 24].

The FSHD-associated DUX4 gene encodes at least two different protein isoforms generated through alternative mRNA splicing (Fig 1B): a non-pathogenic “short” form of unknown function (DUX4-S) expressed at low levels in healthy somatic cells and a longer “full-length” form (DUX4-FL) that is expressed in the male germ line and can be highly cytotoxic when expressed in somatic cells [23, 2528]. Only expression of the DUX4-FL isoform is linked to FSHD [14, 19, 23]. DUX4-fl encodes a DNA-binding transcription factor with a paired homeodomain, and DUX4-FL-specific targets include genes expressed in the germ line and in early development, immune mediators, and retroelements (Fig 1A) [29, 30]. These DUX4-FL targets are misregulated in FSHD and, although the mechanisms are still unclear, it is thought that aberrant expression of one or more of these targets ultimately lead to accumulated muscle pathology [2931].

Interestingly, two proposed alternative FSHD candidate genes, FRG1 (FSHD region gene 1) [32] and FRG2 (FSHD region gene 2) [33], localized proximal to the chromosome 4q35 D4Z4 array, were recently identified as direct DUX4-FL target genes [34, 35], thus linking misexpression of these genes to the widely accepted DUX4 model of FSHD [19]. The molecular function of FRG2 remains unknown; no FRG2 protein has ever been reported and overexpression of the FRG2 mRNA in mice resulted in no apparent phenotype [36]. By contrast, FRG1 is an important for normal development of the vertebrate and invertebrate musculature and vasculature [3639]; overexpression of FRG1 leads to a severe myopathy in mice, adversely affects muscle development and angiogenesis in Xenopus, disrupts muscle structure and organization in C. elegans, and causes primary defects in myogenic stem cells [27, 3640]. However, while some studies reported FRG1 misregulation in FSHD [36, 41, 42], many others failed to find upregulation of FRG1 mRNA or protein in FSHD [4347]. It is possible that FRG1 is only misexpressed in the minor subset of DUX4-fl expressing FSHD myocytes since DUX4-fl expression can directly influence FRG1 expression, which could account for the difficulty in identifying changes in expression levels in patient biopsies. Thus, in addition to DUX4-fl, misexpression of FRG1 may contribute to FSHD pathology and therefore, FRG1 could be a potential therapeutic target for FSHD.

Little is known about the cellular pathways affected by DUX4-FL or FRG1 expression during early development, myogenesis, or in FSHD. We hypothesized that overexpression models generated in a genetically tractable system would provide insight into the pathways affected by DUX4 and FRG1 through the identification of enhancers and suppressors of their functions. DUX4-FL expression consistently leads to apoptosis in somatic cells and adversely affects fertility in vertebrate systems [27, 28, 48, 49], and the apoptotic pathway is highly conserved from invertebrates to human [50, 51]. Thus, although DUX4 is an old world primate-specific gene, a main pathogenic pathway ultimately activated by DUX4-FL expression is conserved. Similarly, the mechanism by which increased expression of FRG1 leads to myopathy is not understood. However, both the sequence and all known biological functions of FRG1 are highly conserved between invertebrates and human [52], suggesting that the myopathic mechanism is also conserved. Drosophila has been used to perform screens for human gene functions by assaying for overexpression phenotypes and the functions of many human genes are highly conserved [53]. In addition, Drosophila has been used successfully to model neuromuscular diseases, including six muscular dystrophies, for investigating pathogenic mechanisms and performing genetic and pharmacologic screens [5463]. Therefore, we generated Drosophila transgenic lines that express DUX4-fl or FRG1 under the control of the GAL4-upstream activation sequence (UAS) [64, 65] to serve as tools to investigate the pathways affected by increased FRG1 or DUX4-FL expression. Importantly, expression of these genes in Drosophila recapitulated the major phenotypes observed in vertebrate systems, apoptosis for DUX4-FL and disrupted musculature for FRG1. In addition, a set of conditions was identified for both the DUX4-fl and FRG1 lines that produce readily screenable phenotypes for potential use in future screens for genetic enhancers and suppressors.

Material and Methods

Drosophila strains

The following fly stocks were obtained from Bloomington Stock Center: DJ667 GAL4 (stock #8171), Act5C-GAL4 (stock #4414), tubP-GAL4 (stock #5138), longGMR-GAL4 (stock 8605), nanos-GAL4:VP16 (stock #7312).

Generation of transgenic lines

A DNA fragment encoding the HA epitope tag (YPYDVPDY) preceded by a start codon was inserted between the EcoRI/BglII sites of the pCaSpeR3 vector [66] to generate pCaSpeR3 HA. The DmFRG1-coding sequence was amplified by PCR from yw cDNA using DmFRG1 5’ BamHI and DmFRG1 3’ XbaI primers (S3 Table) and then subcloned between the BglII/XbaI sites of the pCaSpeR3 HA vector to generate HA-DmFRG1- pCaSpeR3. This plasmid was used to generate UAS-DmFRG1 transgenic lines by standard transformation procedures.

The human DUX4-coding sequence was codon optimized for expression in Drosophila (, and the entire DUX4-flMKG coding sequence was synthesized and subcloned into the pUC57 vector, generating HA-DUX4-flMKG (GenScript USA Inc., S1 Fig). The HA-DUX4-flMKG fragment was subcloned between the NotI/XbaI sites of the UASp or pUAST vectors. The shorter HA-DUX4-flMAL sequence was PCR-amplified from HA-DUX4-flMKG-pUC57 and cloned between the NotI/XbaI sites of the UASp or pUAST vectors. UASp-HA-DUX4-flMKG, pUAST-HA-DUX4-flMKG, UASp-HA-DUX4-flMAL, and pUAST-HA-DUX4-flMAL plasmid DNAs were injected by Duke University Model Systems Genomics Core in 2010 (this service is no longer available), and G0 larvae (the injectees) were sent to our laboratory for further crosses to establish and balance the lines.

Production of FRG1 antibodies

Two DmFRG1 rabbit polyclonal antibodies were generated (GenScript Corporation, Piscataway, NJ) against synthesized peptides targeting amino acid sequences 228–241 for DM1 and 247–262 for DM2 (NP_649202), and then affinity purified prior to use.

Western Blotting

Total protein was extracted from 100 heads/thoraces or embryos in RIPA extraction buffer with protease inhibitors and analyzed (50μg total protein per lane) by SDS-PAGE and western blotting. Both DM1 and DM2 affinity purified antibodies were used at 1:1500 dilution followed by 1:5000 Donkey anti-rabbit-HRP antibody (Roche).


Adult flies with indicated genotypes were collected at 2 days and 10 days after eclosion and kept frozen at -80°C. Each frozen fly was dissected into thorax/legs, abdomen, and head on dry ice, and groups of 40 (20 male and 20 female) were homogenized in TRIzol (Life Technologies) for total RNA extraction as per manufacturer’s instructions. Total RNAs were treated with DNase I on column and purified using the RNeasy mini kit according to the manufacturer’s protocol (QIAGEN). One-step qRT-PCR was performed using 30ng or 15ng of total RNA for DmFRG1 and rp49 expression analysis, respectively (iTaq Universal SYBR Green One-Step Kit, Bio-Rad Laboratories). Cycling conditions were: 50°C for 10 min, 95°C for 1 min, then 40 cycles of 95°C for 10 sec, 60°C for 15 sec, and 72°C for 30 sec. The primers used for qPCR analysis are listed in S3 Table.


Immunofluorescence of ovaries was performed as described with representative images shown [67]. Eye imaginal discs were dissected from 3rd instar larvae and immunostained as described with representative images shown [68]. Adult thoraxes were dissected and fixed in 4% paraformaldehyde/PBS at 4°C for 1 hour, and then cryoprotected in 12% sucrose/PBS at 4°C overnight before being embedded in OCT (Tissue Tek). Cryosections (10-μm thick) were immunostained as described [69]. Antibodies and dilutions used are: rat anti-HA 3F10 (1:200, Roche), mouse anti-ELAV-9F8A9 (1:10), rabbit anti-DmFRG1 DM1 (1:300), rabbit anti-DmFRG1 DM2 (1:300), and Alexa 594 or 488-conjugated secondary antibodies. Nuclei were visualized with DAPI (Invitrogen). Elav-9F8A9 was deposited to the Developmental Studies Hybridoma Bank by G.M. Rubin. For polytene chromosome spreads, salivary glands were dissected from >100 third-instar larvae grown at 25°C and immunofluorescence was performed as described [70].


Newly hatched flies were placed at 29°C incubator for 10 days before fixation in Carnoy’s solution at room temperature for overnight. Whole flies (n = 20) were further processed for paraffin sections as described [71]. Paraffin sections (12 μm-thick) were allowed to dry overnight and stained with hematoxyline and eosin.

Flight assay

Flies were placed at 29°C incubator for 10 days prior to testing. Flight ability was determined by placing 10-day-old flies in a 20-cm glass vial, allowing the flies to climb the sides, and then tapping the vial to dislodge them from the sides of the vial. Flies were scored as having impaired flight ability if they dropped vertically and hit the bottom of the vial instead of flying to catch the side of the tube.


Transgenic lines will be available through the Bloomington Drosophila Stock Center at Indiana University (


Generation and characterization of UAS-DUX4 transgenic lines

Each D4Z4 repeat unit (RU) from the human chromosome 4q35 array contains an open reading frame encoding the DUX4 transcription factor; however, due to the polyadenylation signal residing on a third exon located in the subtelomere distal to the D4Z4 array, only the distal D4Z4 RU produces a stable polyadenylated mRNA and is pathogenic when expressed in myogenic cells [19, 23]. The DUX4-FL coding sequence is contained in a single exon with two potential in-frame methionines that could serve as translation initiation codons: the first at base pair (bp) 4912 (termed the MKG start codon in reference to the first 3 amino acids) and the second at bp 5094 (termed the MAL start codon) using the base alignments from the 5’ KpnI site (bp 1) considered the proximal boundary of the first intact D4Z4 of the lamda42 clone [22, 72]. Mapping of capped mRNA transcripts in myogenic cells identified multiple 5’-capped ends of the DUX4 mRNA located from bps 4941–4962, between MKG and MAL, suggesting that MAL is a functional translation initiation codon in vivo, but not precluding that MKG could be utilized under certain conditions or in other cell types [72]. In fact, the MKG translation initiation site has recently been reported to generate functional protein in human mesenchymal stromal cells [73]. Therefore, we synthesized two DNAs, one encoding the DUX4-FL protein starting from MKG (DUX4-flMKG) and one encoding DUX4-FL from MAL (DUX4-flMAL). Both syntheses were codon optimized for expression in Drosophila and contained a single HA epitope tag at the amino terminus (S1 Fig). The two sequences were cloned into the pUASp [74] and pUAST [64] vectors for germ line and somatic expression, respectively, and each of the four constructs was injected into 125 embryos and analyzed (S1 Table).

Injections of pUAST-DUX4-flMKG and pUAST-DUX4-flMAL transgenes produced very few transgenic flies, which may not be surprising since even low levels of DUX4-FL are highly cytotoxic in vertebrate somatic cells [25, 27, 49], and suggests that this key activity of the human DUX4-FL protein is conserved in Drosophila. Interestingly, there were differences between the two transgenes; pUAST-DUX4-flMAL produced 7 independent transgenic lines, all of which died prior to reproduction, while pUAST-DUX4-flMKG produced 8 transformants, 1 of which died and 7 of which were sterile. Thus, no stable transgenic lines were generated from either DUX4-fl sequence using the pUAST somatic expression vector.

UAS-DUX4-fl transgenic lines were successfully generated using the UASp germline expression vector, with transformants showing 0% mortality. Considering the lethal phenotype generated with the somatic vector, this was surprising since one might expect low-level leaky expression in somatic cells even with the germline vector. Likely the transgenes in these cases inserted into regions of the fly genome that were less favorable to transcription and suppressed their expression allowing for successful embryogenesis. Again, there were differences found between the two constructs; offspring from both were fertile, however, the UAS-DUX4-flMKG transgene produced very weak lines which were ultimately lost, while the UASp-DUX4-flMAL transformants were relatively healthy and two independent lines, UASp-DUX4 #26 (2nd chromosome insertion) and #55 (3rd chromosome insertion) were successfully established and used in the following experiments.

In humans, DUX4-fl is expressed in the male germline of healthy individuals, while expression in the female germline has not been investigated. To determine the effect of DUX4-fl expression on the Drosophila male and female germlines, UASp-DUX4 flies were crossed with nanos (nos) GAL4:VP16, and the testes and ovaries were examined. Neither male nor female nosGAL4:VP16; UASp-DUX4 showed lethality, however, all male nosGAL4:VP16; UASp-DUX4 flies were sterile and had malformed testis (Fig 2 and Table 1). In contrast, female nosGAL4:VP16; UASp-DUX4 flies were fertile and had apparently normal ovaries. Immunostaining confirmed expression of DUX4-FL during oogenesis. We conclude that DUX4-fl expression has sex-specific effects on the Drosophila germline with no adverse effects on the ovaries or female fertility, while the Drosophila testis, as opposed to the case of human males, cannot tolerate DUX4-fl expression.

Fig 2. Effects of DUX4-fl expression on the Drosophila germline.

Adult testis and reproductive tract of nosGAL4:VP16/+ (A and A’) and nosGAL4:VP16/+, UASp-DUX4/+ (B and B’). The nosGAL4:VP16/+ has normally developed testis showing spermatagonia (S) progressing to developing immature sperm (IS) and accumulated mature sperm (MS). The nosGAL4:VP16, UASp-DUX4 male has an extremely small testis with relatively normal accessory gland (AG) and anterior ejaculatory duct (AD). Magnified picture of nosGAL4:VP16, UASp-DUX4 testis (B’) shows lack of fully matured sperm that are observed in normal testis (A’, white arrowheads). Adult ovaries of the nosGAL4:VP16/+ (C) and nosGAL4:VP16/+, UASp-DUX4/+ (D). The nosGAL4:VP16/+, UASp-DUX4/+ ovaries are filled with developing oocytes and are indistinguishable from normal ovaries (C). E and F) Immunostaining of ovariole from nosGAL4:VP16/+, UASp-DUX4/+ shows HA-DUX4-FL (green) is expressed in mid stage of oogenesis (stage 8); DAPI (blue) and phalloidin (red) staining are shown in the overlay. Bar = 500 μm in panels A-D, 100 μm in panels A’ and B’, and 50 μm in panel E.

A Drosophila model of DUX4-fl for identifying genetic interactions

DUX4-fl is highly cytotoxic when expressed in vertebrate somatic cells in culture or during vertebrate embryonic development [25, 27, 28, 75]. Ubiquitous expression of DUX4-fl during development induced by tubulin 1∂ promoter-GAL4 (tubP-GAL4) [76] or Actin5C promoter-GAL4 (Act5C-GAL4) resulted in 100% lethality (Table 1) indicating that this developmental lethal effect is conserved in Drosophila. We attempted to bypass the developmental lethality by inducing DUX4-fl expression at later stages in the adult muscle by using the DJ667 GAL4 line reported to express primarily in adult thoracic muscle [77], however, this cross also resulted in 100% lethality (Table 1). Since we were unable to generate viable flies that expressed DUX4-fl during development or specifically in muscle, we attempted to restrict DUX4 expression to the Drosophila eye, a commonly used model for developmental processes including cell proliferation, cell signaling, and apoptosis [51, 7880] as well as for studying transcription factors [8184]. We crossed UAS-DUX4 lines with the long GMR (lGMR)-GAL4 driver line, which expresses GAL4 in the eye under control of five copies of a 38bp glass-binding site with higher specificity and less robustness than regular GMR-GAL4 that utilizes a shorter glass-binding site [78, 85, 86]. Although lGMR-GAL4 induces transgene expression primarily in the photoreceptors in the eye imaginal disc during third instar larval stage, F1 offspring showed a predominant pupal lethal phenotype (Table 1); the cross between lGMR-Gal4/ lGMR-Gal4 and UASp-DUX4 #26/CyO produced only 5 lGMR-Gal4/ UASp-DUX4 #26 flies while 142 of lGMR-Gal4/CyO were produced. This is likely due to low ectopic expression of DUX4-fl by lGMR-GAL4 in other tissues [87]. Lethality was more pronounced in the F1 males, however, a number of F1 females were born (Table 1) that displayed a readily apparent eye phenotype with 100% penetrance (Fig 3). Immunostaining confirmed DUX4 protein expression in the eye imaginal discs of GMR-GAL4, UAS-DUX4 third instar larvae (Fig 4). Importantly, this DUX4-mediated eye phenotype was distinctly different from those produced by similarly overexpressing other transcription factors in the eye indicating this phenotype was not merely the result of a non-specific effect due to the overexpression of a transcription factor or signaling protein [8084]. We conclude that we have successfully generated a line of transgenic DUX4-fl Drosophila that can be crossed to generate a model that can be utilized for genetic screening to identify potential genetic enhancers and suppressors of DUX4-FL function.

Fig 3. Ectopic DUX4-fl expression by lGMR-GAL4 produces a readily screenable eye phenotype.

A-C) Compound eyes of lGMR-GAL4 consist of precisely organized and pigmented ommatidia and bristles. D-F) Eyes of lGMR-GAL4/+, UASp-DUX4/+ are the usual size but lack organized ommatidia. Corneal lenses and pigment cells are completely missing; bristles are formed, but irregularly dispersed. Bar = 100 μm in panel D; Bar = 50 μm in panels E and F.

Fig 4. Expression of DUX4-FL in eye imaginal disc leads to disruption of eye formation.

Third instar eye imaginal discs from A) lGMR-GAL4/+ or B and C) lGMR-GAL4/+; UASp-DUX4/+ were immunostained for the photoreceptor marker ELAV (green) or HA-DUX4 (red), and stained for DAPI (blue). C) Expression of DUX4-FL protein was detected in mature photoreceptors posterior to the morphogenetic furrow. Bar = 50 μm and 10 μm in the magnified picture.

Generation and characterization of Drosophila transgenic lines of UAS-DmFRG1

In humans, aberrant upregulation of FRG1 expression, via epigenetic dysregulation of the FSHD-associated chromosome 4q35 region and, as recently discovered, through the binding of DUX4-FL, has long been a proposed disease mechanism for FSHD [36, 41, 88]. Overexpression of FRG1 or its orthologs in mouse, Xenopus, and C. elegans inhibits myogenic cell migration, leads to defects in myogenic stem cells, disrupts muscle development and function, and recapitulates many features of FSHD [3640], however the specific pathways leading to these phenotypes are not known. In contrast to primate-specific DUX4, human FRG1 at chromosome 4q35 is highly conserved in metazoans, including Drosophila, across its entire open reading frame [32, 52, 89]. Drosophila FRG1 (DmFRG1; CG6480) exhibits 50% amino acid identity (66% similarity) with its human ortholog and contains similar functional domains (Fig 5A); therefore, we hypothesized that the Drosophila and human FRG1 proteins likely have a conserved biological function and Drosophila would be a suitable system for identifying conserved FRG1 affected pathways.

Fig 5. FRG1 is highly conserved between human and Drosophila.

(A) Alignment of the predicted amino acid sequence for the human (Hs) and D. melanogaster (Dm) FRG1 orthologs. Conserved amino acids are highlighted in yellow with identical amino acids indicated by the letter and similar amino acids indicated by a +. The functional domains, including the nuclear localization signals (NLS) and RNA binding domain (RBD), are indicated. The peptides used as antigens for generating the DM1 and DM2 antibodies are boxed in red. (B) DmFRG1 expression was assayed by qRT-PCR at day 2 (D2) and day 10 (D10) in the thorax or head and abdomen combined, as indicated. Expression was normalized to rp49 RNA levels and presented as fold expression compared to D2 or D10 thorax. Induction of DmFRG1 mRNA was significant (* p < 0.01 by Student’s t-test) for both lines when compared with w and DJ667GAL4 alone. (C) Left panel: Western blots of protein extracts from 0–17h embryos (lane 1 and 4) or head/thorax of adult flies (lanes 2, 3, 5, and 6) of yw strain (lanes 1, 2, 4, and 5) or tubP-GAL4,UAS-DmFRG1 flies (lanes 3 and 6), probed with the DM1 or DM2 antibody as indicated. Beta-tubulin was used as a loading control. (D) Thoracic muscle tissue immunostained for DmFRG1 (green) and counterstained with DAPI (blue) and phalloidin (red). Endogenous DmFRG1 is not detectable in the nuclei of yw flies (white arrows) and accumulates in nuclei when overexpressed (yellow arrows). Zoomed regions displayed in the lower panels are outlined in the upper panels by dotted white boxes.

We aimed to use Drosophila to create a genetic tool that could be used to identify and better understand the cellular pathways disrupted by FRG1 overexpression, and which therefore might play roles in FSHD pathogenesis. Transgenic Drosophila lines containing the coding sequence of DmFRG1 with an HA epitope tag at the amino terminus were generated using the pUAST vector [64]. Since FSHD predominantly affects adult muscles and the human FRG1 gene is a direct transcriptional target of the DUX4-FL protein in FSHD muscle [34], the UAS-DmFRG1 flies were crossed with the DJ667 GAL4 line, which expresses GAL4 predominantly in adult thoracic muscle [77]. Our qRT-PCR analysis confirmed that DJ667 GAL4, DmFRG1 flies showed increased FRG1 expression predominantly in thoracic muscle as they aged (Fig 5B). With UAS-DmFRG1 line 11, there was a 5-fold overexpression of DmFRG1 mRNA 2 days after hatching that increased to 17-fold at 10 days; with line 12, expression increased from 32-fold to 50-fold. Both double transgenic lines were viable and fertile.

Tissues from yw and UAS-DmFRG1 adult flies were also assayed for FRG1 protein expression using two affinity-purified polyclonal antibodies (DM-1 and DM-2) generated against the carboxyl terminus of DmFRG1 (Fig 5A). These antibodies detect both the endogenous DmFRG1 protein and the transgenic overexpressed protein (Fig 5C). The transgenic DmFRG1 has an amino terminal HA epitope tag that allows differential detection of endogenous and overexpressed DmFRG1 (Fig 5C). In vertebrates, FRG1 has multiple distinct subcellular localizations: a nuclear pool associated with nascent mRNA transcripts on the chromatin and nucleoli, and a cytoplasmic protein pool [90, 91]. Interestingly, in all model systems we tested previously, endogenous FRG1 was predominantly, but not exclusively, cytoplasmic and the overexpression of FRG1 led to preferential accumulation in the nucleus, and particularly in the nucleolus, suggesting that FRG1 protein levels affect subcellular localization and are likely to be tightly regulated [90, 91]. Immunostaining for DmFRG1 in Drosophila muscle and salivary tissues showed a similar pattern (Figs 5D and 6A–6G). As with overexpression in vertebrate cell culture, all detectable DmFRG1 expressed from the transgene was nuclear in tubP-GAL4, UAS-DmFRG1 salivary glands (Fig 6, compare panels E and F). In the nuclear pool of DmFRG1, the overexpressed and endogenous proteins had similar, overlapping subnuclear localization profiles (Fig 6G). The FRG1 associated with polytene chromosomes preferentially localized to the DAPI-poor euchromatic puffs (Fig 6L and 6M), and the overexpressed DmFRG1 showed overlapping localization with the endogenous chromatin-associated DmFRG1 (Fig 6K). Overall, based on this preliminary examination, DmFRG1 behaves similar to its vertebrate orthologs.

Fig 6. Nuclear localization of endogenous and overexpressed DmFRG1 is conserved.

Salivary gland tissue (A-G) and polytene chromosome spreads (H-M) from w (A, B) and tubP-GAL4, UAS-DmFRG1 were immunostained for total DmFRG1 using the DM2 antibody (red; A-E, G, I, K, L) or specifically overexpressed DmFRG1 using the HA antibody (green; F, G, J, K, M), and stained with DAPI (blue) to show the nuclei (A, C) or chromosomes (H, L, M). Endogenous DmFRG1 is predominantly cytoplasmic (A, B), while overexpressed DmFRG1 accumulates in the nucleus (E, F, G). In the nucleus, the endogenous and overexpressed DmFRG1 localizations mostly overlap (yellow; G, K).

Overexpression of DmFRG1 in adult muscle disrupts organization of the musculature and impairs muscle function

FSHD is typically an adult onset progressive myopathy leading to decreased skeletal muscle mass and ultimately loss of muscle function. FRG1 expression is moderately induced by the DUX4-FL transcription factor in human myocytes due to a human specific DUX4-FL responsive intronic enhancer [92], and overexpression of FRG1 in muscle results in an FSHD-like myopathy in mice and impaired muscle development, function, and movement in Xenopus and C. elegans [3638, 93]. Therefore, we generated flies overexpressing DmFRG1 in the adult musculature and assayed them for a basic muscle function: the ability to fly (S1 Movie 1 and 2). The parent lines DJ667 GAL4 and UAS-DmFRG1, which express wild-type levels of DmFRG1, are capable of movement and flight indistinguishable from yw flies. However, their progeny overexpressing DmFRG1 in adult thoracic muscles have substantially impaired flight ability (Summarized in S2 Table). These DJ667 GAL4, UAS-DmFRG1 flies have fully developed wings, are capable of walking normally and jumping for takeoff, but were nonetheless incapable of sustained flight (S2 Movie). Thus, overexpression of DmFRG1 in flight muscles resulted in impaired function.

Overexpression of FRG1 disrupts the organization and integrity of the musculature in other model organisms and muscle from FRG1 overexpressing mice show features of muscular dystrophy [3638]. Thus, the thoracic muscles of DmFRG1 overexpressing flies were analyzed histologically and compared with controls for similar indications (Fig 7). Hematoxylin and eosin (H&E) staining of thoraces revealed that DmFRG1 overexpression leads to a disorganized musculature. The dorsal longitudinal muscles (DLMs) in control flies exhibited the typical pattern of 12 organized bundles, six on each side (Fig 7A), however, DLMs from the DmFRG1 overexpressing flies were misshapen, fused together, and were overall highly disorganized (Fig 7B) [58]. Analysis of the dorso-ventral muscle bundles suggested muscle degeneration in the tergosternal muscles (indirect with levator muscles) (Fig 7D). Overall, overexpression of DmFRG1 disrupts the integrity of the musculature and impairs muscle function. We conclude that we have successfully generated a model of FRG1-mediated muscle dysfunction that is readily amenable to screening for modifiers of the phenotype.

Fig 7. Abnormal musculature in DM-FRG1 overexpressing flies.

H&E stained paraffin sections of thoraces from DJ667GAL4 (A and C) and of DJ667GAL4; DmFRG1 (B and D) adult flies. (B) Overexpression of DmFRG1 leads to disorganized dorsal longitudinal muscles (DLMs, indirect wing depressors) exhibiting variable numbers and shapes of muscles suggestive of muscle degeneration (arrowheads) compared with the highly organized musculature observed in the controls (A), which exhibit the characteristic 6 distinct DLMs on each side. (C and D) H&E stained paraffin sections of the dorso-ventral tergosternal muscle bundles (indirect wing levators) show histological features characteristic of muscle degeneration (arrowheads). * denotes the same muscle in these flies for a reference. Bar = 500 μm.


The FSHD pathogenic mechanisms downstream of DUX4-fl misexpression are not well understood due in large part to a lack of phenotypic DUX4-based FSHD-like animal models. Circumventing DUX4-fl cytotoxicity and lethality during early development has been a major hurdle inhibiting the generation of viable transgenic FSHD models since even trace amount of spurious DUX4-fl transcription during embryogenesis can be lethal. In fact, generating the only viable transgenic mouse line that expresses DUX4-fl mRNA, the D4Z4-2.5 mice, required more than 450 injections to obtain one viable and fertile line [94], mirroring the situation we faced while generating the Drosophila DUX4 lines. Compounding the problem, the DUX4 gene evolved relatively recently and is specific to old-world primates. DUX4 originated from a gene conversion event in the mammalian DUXC macrosatellite array that occurred in the primate and Afrotheria lineages, and subsequently translocated to chromosome 4qter in primates [95, 96]. Therefore, despite apparent homology to ancestral paired homeodomain transcription factors, which is restricted to the DNA binding domains, traditional model systems such as mice, rats, flies, and zebrafish do not have true parental DUX4 orthologs and no natural models exist [95] and one must always consider potential nonspecific effects when working with DUX4 expressed in non-human systems.

Although generally silent in adult somatic tissues, DUX4-fl is expressed normally in human testis, pluripotent stem cells [23], and many somatic tissues of FSHD1 and healthy fetuses, suggesting that the DUX4 retrogene has likely evolved to function specifically during primate germ line and embryonic development [97, 98]. Presumably, the DUX4-FL protein co-opted the host primate genome and cellular machinery to regulate certain endogenous primate genes and cellular pathways [2931]. Thus, despite DUX4 being primate-specific, most of the DUX4-FL target genes and affected pathways are evolutionarily conserved and present in model organisms, allowing introduction of DUX4-FL to produce a potentially useful model of certain aspects of FSHD. In fact, Xenopus and zebrafish embryos injected with DUX4-fl mRNA and mice expressing DUX4-fl via viral infection or transgene expression exhibit phenotypes consistent with FSHD [27, 28, 75, 99]. One caveat is that although many protein-coding DUX4-FL target genes are conserved, their regulatory elements may not be conserved, resulting in gene expression patterns that do not fully overlap with FSHD transcription profiles or those of human cells expressing exogenous DUX4-fl [29, 31, 100]. For example, the human FRG1 gene contains a functional intronic DUX4-FL binding site but this site is absent from the murine Frg1 gene, rendering it non-inducible by DUX4-FL [92].

A key part of DUX4 evolution in primates includes the silencing of DUX4-fl expression in adult somatic tissues, where its expression is deleterious. Upon loss of epigenetic silencing in FSHD, abnormal DUX4-fl expression in adult skeletal muscle has pathological consequences by aberrantly activating target genes and DUX4-regulated cellular pathways [31]. Low levels of DUX4-FL are highly cytotoxic when expressed in somatic cells and DUX4-FL expression disrupts vertebrate development [25, 27, 28, 49, 75]. This phenotype is conserved in our Drosophila DUX4 model as evidenced by the difficulty in generating transgenic DUX4 lines and the observed phenotypes. Although clinical symptoms of FSHD manifest in adult skeletal muscles, DUX4-fl expression was lethal at the levels dictated by the muscle or ubiquitous GAL4 drivers, and we only obtained viable and fertile flies when expression was restricted to the developing eye. Fortunately this expression pattern still produced a cellular phenotype consistent with FSHD. However, in addition to the eye phenotype, the developmental lethality induced from the ubiquitous Act5c-GAL4 and tubP-GAL4 crosses is another screenable phenotype for DUX4 genetic interactions that may be more relevant in other tissues. Thus, we have generated a viable Drosophila model of DUX4 expression that can be utilized to generate flies that are readily screenable for suppressors or enhancers of the phenotype, the results of which would be of great interest to the FSHD field.

Two myogenic enhancers proximal to the FSHD-associated 4q35 D4Z4 array were recently identified and shown to regulate DUX4 in differentiated skeletal myocytes [101], providing a potential explanation for the relatively muscle-specific pathology seen in FSHD. In addition, FRG1, a transcriptional target of DUX4-FL in humans, produces a myopathic phenotype generally consistent with FSHD when overexpressed in muscle [3638]. We have now generated transgenic Drosophila lines that, when crossed with an adult muscle-specific GAL4 driver, produce a model of FRG1-mediated muscle dysfunction that recapitulates many aspects of the FSHD phenotype. In addition, FRG1 plays a critical role in both myogenesis and angiogenesis. Crossing to additional GAL4 drivers or performing enhancer/suppressor screens may prove useful in determining the normal biological functions of FRG1 in these tissues, some of which may be relevant to FSHD.

Informative Drosophila models have been generated for several neuromuscular diseases and for six of the nine classes of muscular dystrophy including Duchenne [58, 61], myotonic [57, 102], congenital, including certain dystroglycanopathies [58, 59, 103, 104], Emery-Dreyfus [60, 105], oculopharyngeal [56], and limb-girdle [54]; however, no Drosophila model for FSHD based on any candidate gene has been reported. Therefore, the Drosophila lines presented here that will allow investigations into the functions of two genes important to FSHD and will fill an important void in FSHD research by providing valuable resources for those studying muscle development and FSHD.


The primary mediator of FSHD pathophysiology is the aberrant stable expression of the DUX4-fl mRNA isoform in adult somatic cells. Expression of DUX4-FL in somatic cells can initiate many potentially adverse downstream events including changes in gene expression, disruption of RNA and protein metabolism, and the induction of apoptosis. However, little is known about the precise pathways affected by DUX4-FL expression and it is still not known which DUX4-mediated changes lead to FSHD pathology. FRG1 has been proposed to be involved in FSHD, as it is a direct transcriptional target of DUX4-FL, and its overexpression causes a myopathic phenotype in mice through an unknown mechanism. Thus, there is a need in the FSHD field for genetically tractable model organisms to investigate the cellular pathways disrupted by aberrant DUX4-FL and FRG1 expression and to determine which of these pathways are potentially involved in pathogenesis. FRG1 is very highly conserved between Drosophila and human and readily amenable to model systems approaches. DUX4, however, is primate specific and not conserved in Drosophila, and thus is reliant on conservation of the relevant cellular machinery and pathways; successful DUX4-based models have been generated in Xenopus and Zebrafish despite their lack of DUX4 orthologs. Therefore, we generated transgenic lines of Drosophila expressing DUX4-fl or FRG1 under the control of the GAL4-UAS system that produced readily screenable phenotypes consistent with what is known about the functions of these proteins in other systems. Induction of DUX4-fl expression during early development was lethal and expression in the eye imaginal disc produced resulted in white ommatidia and disorganized bristles in the adult eye. Induction of FRG1 in the thoracic muscles leads to a disorganized musculature and impaired flight ability. These Drosophila phenotypes will be valuable tools for performing genetic screens to identify components of the DUX4-fl apoptotic pathway and the developmental pathways disrupted by FRG1 expression in muscle. In addition, Drosophila models based on human disease genes, including many muscular dystrophies, have been used to discover underlying disease mechanisms and for drug screens to identify potentially therapeutic compounds. The DUX4 and FRG1 transgenic flies reported here will provide the tools for similar investigations into mechanisms of FSHD.

Supporting Information

S1 Fig. Sequence of the codon optimized DUX4-fl open reading frame.

The sequence of the DUX4-fl cDNA was codon optimized for expression in Drosophila melanogaster and synthesized in vitro. Changed nucleotides are indicated in red. * indicates translational stop codon.


S1 Movie. Increased FRG1 expression in adult muscle impairs flight (Part 1).

Groups of flies were analyzed for the ability to fly. Flies were forcibly dislodged from the surface of a vial and scored for their ability to prevent themselves from falling to the bottom by flying. Those that fell were scored as unable to fly; those that immediately lit upon the sides of the vials did so via flight, thus preventing themselves from falling, and were scored as capable of flying. The adult muscle GAL4 driver strain DJ667 (left) and the UAS-DmFRG1 strain (right) were readily able to flying upon being dislodged and return to the sides of the vial. However, the DJ667 GAL4, UAS-DmFRG1 progeny (middle), which produced flies overexpressing DmFRG1 in their adult muscles, were unable to fly and fell to the bottom of the vial when dislodged.


S2 Movie. Increased FRG1 expression in adult muscle impairs flight (Part 2).

A representative adult DJ667,UAS-DmFRG1 fly, which overexpresses DmFRG1 in its thoracic muscles, appears normal and is capable of walking and flexing its intact wings but is unable to fly. These flies jump into the air for take-off as per usual, however, instead of flying they fall back down immediately.


S2 Table. Overexpression of DmFRG1 in adult thorax impairs flight ability.


S3 Table. Oligonucleotides used for cloning and qPCR.



The authors thank Dr. Charis Himeda for valuable discussions and help writing the manuscript, Dr. Huey Hing for help generating the DmFRG1 transgenic flies, Dr. Richard Cripps for his technical advice, and the Chris Carrino Foundation for FSHD, the Association Française contra les Myopathies, the Muscular Dystrophy Association, and the FSH Society for their continued support of our FSHD research programs.

Author Contributions

Conceived and designed the experiments: TIJ PLJ. Performed the experiments: TIJ MP PLJ. Analyzed the data: TIJ MP PLJ. Wrote the paper: TIJ PLJ.


  1. 1. Deenen JC, Arnts H, van der Maarel SM, Padberg GW, Verschuuren JJ, Bakker E, et al. Population-based incidence and prevalence of facioscapulohumeral dystrophy. Neurology. 2014;83:1056–9. pmid:25122204.
  2. 2. Orphanet. Prevalence of rare diseases: Bibliographic data in Orphanet Report Series: Rare Diseases Collection: Inserm; 2011 [May 2011]. Available:
  3. 3. Padberg GW. Facioscapulohumeral Disease [thesis]. Leiden, the Netherlands: Leiden University; 1982.
  4. 4. Tawil R, Van Der Maarel SM. Facioscapulohumeral muscular dystrophy. Muscle Nerve. 2006;34(1):1–15. Epub 2006/03/02. pmid:16508966.
  5. 5. de Greef JC, Lemmers RJ, Camano P, Day JW, Sacconi S, Dunand M, et al. Clinical features of facioscapulohumeral muscular dystrophy 2. Neurology. 2010;75(17):1548–54. Epub 2010/10/27. 75/17/1548 [pii] pmid:20975055.
  6. 6. Brouwer OF, Padberg GW, Wijmenga C, Frants RR. Facioscapulohumeral muscular dystrophy in early childhood. Arch Neurol. 1994;51(4):387–94. Epub 1994/04/01. pmid:8155016.
  7. 7. Klinge L, Eagle M, Haggerty ID, Roberts CE, Straub V, Bushby KM. Severe phenotype in infantile facioscapulohumeral muscular dystrophy. Neuromuscul Disord. 2006;16(9–10):553–8. Epub 2006/08/29. S0960-8966(06)00436-6 [pii] pmid:16934468.
  8. 8. Nikolic A, Ricci G, Sera F, Bucci E, Govi M, Mele F, et al. Clinical expression of facioscapulohumeral muscular dystrophy in carriers of 1–3 D4Z4 reduced alleles: experience of the FSHD Italian National Registry. BMJ open. 2016;6(1):e007798. pmid:26733561; PubMed Central PMCID: PMC4716236.
  9. 9. Tawil R, Forrester J, Griggs RC, Mendell J, Kissel J, McDermott M, et al. Evidence for anticipation and association of deletion size with severity in facioscapulohumeral muscular dystrophy. The FSH-DY Group. Ann Neurol. 1996;39(6):744–8. pmid:8651646.
  10. 10. Zatz M, Marie SK, Cerqueira A, Vainzof M, Pavanello RC, Passos-Bueno MR. The facioscapulohumeral muscular dystrophy (FSHD1) gene affects males more severely and more frequently than females. Am J Med Genet. 1998;77(2):155–61. pmid:9605290.
  11. 11. Ricci E, Galluzzi G, Deidda G, Cacurri S, Colantoni L, Merico B, et al. Progress in the molecular diagnosis of facioscapulohumeral muscular dystrophy and correlation between the number of KpnI repeats at the 4q35 locus and clinical phenotype. Ann Neurol. 1999;45(6):751–7. pmid:10360767.
  12. 12. Wohlgemuth M, Lemmers RJ, van der Kooi EL, van der Wielen MJ, van Overveld PG, Dauwerse H, et al. Possible phenotypic dosage effect in patients compound heterozygous for FSHD-sized 4q35 alleles. Neurology. 2003;61(7):909–13. Epub 2003/10/15. pmid:14557558.
  13. 13. Ricci G, Scionti I, Ali G, Volpi L, Zampa V, Fanin M, et al. Rippling muscle disease and facioscapulohumeral dystrophy-like phenotype in a patient carrying a heterozygous CAV3 T78M mutation and a D4Z4 partial deletion: Further evidence for "double trouble" overlapping syndromes. Neuromuscul Disord. 2012. Epub 2012/01/17. S0960-8966(11)01406-4 [pii] pmid:22245016.
  14. 14. Jones TI, Chen JC, Rahimov F, Homma S, Arashiro P, Beermann ML, et al. Facioscapulohumeral muscular dystrophy family studies of DUX4 expression: evidence for disease modifiers and a quantitative model of pathogenesis. Hum Mol Genet. 2012;21(20):4419–30. Epub 2012/07/17. dds284 [pii] pmid:22798623; PubMed Central PMCID: PMC3459465.
  15. 15. Lemmers RJ, Goeman JJ, Van Der Vliet PJ, Van Nieuwenhuizen MP, Balog J, Vos-Versteeg M, et al. Inter-individual differences in CpG methylation at D4Z4 correlate with clinical variability in FSHD1 and FSHD2. Hum Mol Genet. 2015;24(3):659–69. Epub 2014 Sep 25. pmid:25256356.
  16. 16. Jones TI, King OD, Himeda CL, Homma S, Chen JC, Beermann ML, et al. Individual epigenetic status of the pathogenic D4Z4 macrosatellite correlates with disease in facioscapulohumeral muscular dystrophy. Clinical epigenetics. 2015;7(1):37. pmid:25904990; PubMed Central PMCID: PMC4405830.
  17. 17. Himeda CL, Jones TI, Jones PL. Facioscapulohumeral muscular dystrophy as a model for epigenetic regulation and disease. Antioxidants & redox signaling. 2015;22(16):1463–82. Epub 2014 Dec 4. pmid:25336259; PubMed Central PMCID: PMCPMC4432493.
  18. 18. de Greef JC, Lemmers RJ, van Engelen BG, Sacconi S, Venance SL, Frants RR, et al. Common epigenetic changes of D4Z4 in contraction-dependent and contraction-independent FSHD. Hum Mutat. 2009;30(10):1449–59. Epub 2009/09/04. pmid:19728363.
  19. 19. Lemmers RJ, van der Vliet PJ, Klooster R, Sacconi S, Camano P, Dauwerse JG, et al. A unifying genetic model for facioscapulohumeral muscular dystrophy. Science. 2010;329(5999):1650–3. Epub 2010/08/21. science.1189044 [pii] pmid:20724583.
  20. 20. Sacconi S, Lemmers RJ, Balog J, van der Vliet PJ, Lahaut P, van Nieuwenhuizen MP, et al. The FSHD2 gene SMCHD1 is a modifier of disease severity in families affected by FSHD1. Am J Hum Genet. 2013;93(4):744–51. pmid:24075187.
  21. 21. Daxinger L, Tapscott SJ, van der Maarel SM. Genetic and epigenetic contributors to FSHD. Curr Opin Genet Dev. 2015;33:56–61. pmid:26356006.
  22. 22. Gabriels J, Beckers MC, Ding H, De Vriese A, Plaisance S, van der Maarel SM, et al. Nucleotide sequence of the partially deleted D4Z4 locus in a patient with FSHD identifies a putative gene within each 3.3 kb element. Gene. 1999;236(1):25–32. Epub 1999/08/06. S0378-1119(99)00267-X [pii]. pmid:10433963.
  23. 23. Snider L, Geng LN, Lemmers RJ, Kyba M, Ware CB, Nelson AM, et al. Facioscapulohumeral dystrophy: incomplete suppression of a retrotransposed gene. PLoS Genet. 2010;6(10):e1001181. Epub 2010/11/10. pmid:21060811; PubMed Central PMCID: PMC2965761.
  24. 24. Tawil R, van der Maarel SM, Tapscott SJ. Facioscapulohumeral dystrophy: the path to consensus on pathophysiology. Skelet Muscle. 2014;4:12. pmid:24940479; PubMed Central PMCID: PMC4060068.
  25. 25. Kowaljow V, Marcowycz A, Ansseau E, Conde CB, Sauvage S, Matteotti C, et al. The DUX4 gene at the FSHD1A locus encodes a pro-apoptotic protein. Neuromuscul Disord. 2007;17(8):611–23. Epub 2007/06/26. S0960-8966(07)00121-6 [pii] pmid:17588759.
  26. 26. Bosnakovski D, Daughters RS, Xu Z, Slack JM, Kyba M. Biphasic myopathic phenotype of mouse DUX, an ORF within conserved FSHD-related repeats. PLoS One. 2009;4(9):e7003. Epub 2009/09/17. pmid:19756142; PubMed Central PMCID: PMC2737622.
  27. 27. Wuebbles RD, Long SW, Hanel ML, Jones PL. Testing the effects of FSHD candidate gene expression in vertebrate muscle development. Int J Clin Exp Pathol. 2010;3(4):386–400. Epub 2010/05/22. pmid:20490329; PubMed Central PMCID: PMC2872745.
  28. 28. Wallace LM, Garwick SE, Mei W, Belayew A, Coppee F, Ladner KJ, et al. DUX4, a candidate gene for facioscapulohumeral muscular dystrophy, causes p53-dependent myopathy in vivo. Ann Neurol. 2011;69(3):540–52. Epub 2011/03/30. pmid:21446026.
  29. 29. Geng LN, Yao Z, Snider L, Fong AP, Cech JN, Young JM, et al. DUX4 activates germline genes, retroelements, and immune mediators: Implications for facioscapulohumeral dystrophy. Dev Cell. 2012;22(1):38–51. Epub 2012/01/03. S1534-5807(11)00523-5 [pii] pmid:22209328.
  30. 30. Young JM, Whiddon JL, Yao Z, Kasinathan B, Snider L, Geng LN, et al. DUX4 binding to retroelements creates promoters that are active in FSHD muscle and testis. PLoS Genet. 2013;9(11):e1003947. pmid:24278031; PubMed Central PMCID: PMC3836709.
  31. 31. Yao Z, Snider L, Balog J, Lemmers RJ, Van Der Maarel SM, Tawil R, et al. DUX4-induced gene expression is the major molecular signature in FSHD skeletal muscle. Hum Mol Genet. 2014;23(20):5342–52. pmid:24861551; PubMed Central PMCID: PMCPMC4168822.
  32. 32. van Deutekom JC, Lemmers RJ, Grewal PK, van Geel M, Romberg S, Dauwerse HG, et al. Identification of the first gene (FRG1) from the FSHD region on human chromosome 4q35. Hum Mol Genet. 1996;5(5):581–90. pmid:8733123.
  33. 33. Rijkers T, Deidda G, van Koningsbruggen S, van Geel M, Lemmers RJ, van Deutekom JC, et al. FRG2, an FSHD candidate gene, is transcriptionally upregulated in differentiating primary myoblast cultures of FSHD patients. J Med Genet. 2004;41(11):826–36. pmid:15520407.
  34. 34. Ferri G, Huichalaf CH, Caccia R, Gabellini D. Direct interplay between two candidate genes in FSHD muscular dystrophy. Hum Mol Genet. 2015;24(5):1256–66. pmid:25326393; PubMed Central PMCID: PMC4321439.
  35. 35. Thijssen PE, Balog J, Yao Z, Pham TP, Tawil R, Tapscott SJ, et al. DUX4 promotes transcription of FRG2 by directly activating its promoter in facioscapulohumeral muscular dystrophy. Skel Musc. 2014;4(19):1–9.
  36. 36. Gabellini D, D'Antona G, Moggio M, Prelle A, Zecca C, Adami R, et al. Facioscapulohumeral muscular dystrophy in mice overexpressing FRG1. Nature. 2006;439(7079):973–7. pmid:16341202.
  37. 37. Liu Q, Jones TI, Tang VW, Brieher WM, Jones PL. Facioscapulohumeral muscular dystrophy region gene-1 (FRG-1) is an actin-bundling protein associated with muscle-attachment sites. J Cell Sci. 2010;123(Pt 7):1116–23. Epub 2010/03/11. jcs.058958 [pii] pmid:20215405; PubMed Central PMCID: PMC2844320.
  38. 38. Hanel ML, Wuebbles RD, Jones PL. Muscular dystrophy candidate gene FRG1 is critical for muscle development. Dev Dyn. 2009;238(6):1502–12. Epub 2008/12/20. pmid:19097195; PubMed Central PMCID: PMC2964887.
  39. 39. Wuebbles RD, Hanel ML, Jones PL. FSHD region gene 1 (FRG1) is crucial for angiogenesis linking FRG1 to facioscapulohumeral muscular dystrophy-associated vasculopathy. Dis Model Mech. 2009;2(5–6):267–74. Epub 2009/04/23. dmm.002261 [pii] pmid:19383939; PubMed Central PMCID: PMC2675802.
  40. 40. Xynos A, Neguembor MV, Caccia R, Licastro D, Nonis A, Di Serio C, et al. Overexpression of facioscapulohumeral muscular dystrophy region gene 1 causes primary defects in myogenic stem cells. J Cell Sci. 2013;126(Pt 10):2236–45. pmid:23525014.
  41. 41. Bodega B, Ramirez GD, Grasser F, Cheli S, Brunelli S, Mora M, et al. Remodeling of the chromatin structure of the facioscapulohumeral muscular dystrophy (FSHD) locus and upregulation of FSHD-related gene 1 (FRG1) expression during human myogenic differentiation. BMC Biol. 2009;7:41. Epub 2009/07/18. 1741-7007-7-41 [pii] pmid:19607661.
  42. 42. Gabellini D, Green MR, Tupler R. Inappropriate gene activation in FSHD: a repressor complex binds a chromosomal repeat deleted in dystrophic muscle. Cell. 2002;110(3):339–48. pmid:12176321.
  43. 43. Klooster R, Straasheijm K, Shah B, Sowden J, Frants R, Thornton C, et al. Comprehensive expression analysis of FSHD candidate genes at the mRNA and protein level. Eur J Hum Genet. 2009;17(12):1615–24. Epub 2009/10/08. ejhg200962 [pii] pmid:19809486.
  44. 44. Homma S, Chen JC, Rahimov F, Beermann ML, Hanger K, Bibat GM, et al. A unique library of myogenic cells from facioscapulohumeral muscular dystrophy subjects and unaffected relatives: family, disease and cell function. Eur J Hum Genet. 2012;20(4):404–10. Epub 2011/11/24. ejhg2011213 [pii] pmid:22108603; PubMed Central PMCID: PMC3306860.
  45. 45. Osborne RJ, Welle S, Venance SL, Thornton CA, Tawil R. Expression profile of FSHD supports a link between retinal vasculopathy and muscular dystrophy. Neurology. 2007;68(8):569–77. pmid:17151338.
  46. 46. Tsumagari K, Chang SC, Lacey M, Baribault C, Chittur SV, Sowden J, et al. Gene expression during normal and FSHD myogenesis. BMC Med Genomics. 2011;4(1):67. Epub 2011/09/29. 1755-8794-4-67 [pii] pmid:21951698.
  47. 47. Winokur ST, Chen YW, Masny PS, Martin JH, Ehmsen JT, Tapscott SJ, et al. Expression profiling of FSHD muscle supports a defect in specific stages of myogenic differentiation. Hum Mol Genet. 2003;12(22):2895–907. pmid:14519683.
  48. 48. Dixit M, Ansseau E, Tassin A, Winokur S, Shi R, Qian H, et al. DUX4, a candidate gene of facioscapulohumeral muscular dystrophy, encodes a transcriptional activator of PITX1. Proc Natl Acad Sci U S A. 2007;104(46):18157–62. Epub 2007/11/07. 0708659104 [pii] pmid:17984056.
  49. 49. Bosnakovski D, Xu Z, Gang EJ, Galindo CL, Liu M, Simsek T, et al. An isogenetic myoblast expression screen identifies DUX4-mediated FSHD-associated molecular pathologies. EMBO J. 2008;27(20):2766–79. Epub 2008/10/04. emboj2008201 [pii] pmid:18833193.
  50. 50. Fuchs Y, Steller H. Programmed cell death in animal development and disease. Cell. 2011;147(4):742–58. pmid:22078876.
  51. 51. Xu D, Woodfield SE, Lee TV, Fan Y, Antonio C, Bergmann A. Genetic control of programmed cell death (apoptosis) in Drosophila. Fly. 2009;3(1):78–90. pmid:19182545; PubMed Central PMCID: PMC2702463.
  52. 52. Grewal PK, Todd LC, van der Maarel S, Frants RR, Hewitt JE. FRG1, a gene in the FSH muscular dystrophy region on human chromosome 4q35, is highly conserved in vertebrates and invertebrates. Gene. 1998;216(1):13–9. pmid:9714712.
  53. 53. Xu R, Deng K, Zhu Y, Wu Y, Ren J, Wan M, et al. A large-scale functional approach to uncover human genes and pathways in Drosophila. Cell Res. 2008;18(11):1114–27. pmid:18957936.
  54. 54. Allikian MJ, Bhabha G, Dospoy P, Heydemann A, Ryder P, Earley JU, et al. Reduced life span with heart and muscle dysfunction in Drosophila sarcoglycan mutants. Hum Mol Genet. 2007;16(23):2933–43. pmid:17855453.
  55. 55. Chan YB, Miguel-Aliaga I, Franks C, Thomas N, Trulzsch B, Sattelle DB, et al. Neuromuscular defects in a Drosophila survival motor neuron gene mutant. Hum Mol Genet. 2003;12(12):1367–76. pmid:12783845.
  56. 56. Chartier A, Benoit B, Simonelig M. A Drosophila model of oculopharyngeal muscular dystrophy reveals intrinsic toxicity of PABPN1. EMBO J. 2006;25(10):2253–62. pmid:16642034; PubMed Central PMCID: PMC1462976.
  57. 57. de Haro M, Al-Ramahi I, De Gouyon B, Ukani L, Rosa A, Faustino NA, et al. MBNL1 and CUGBP1 modify expanded CUG-induced toxicity in a Drosophila model of myotonic dystrophy type 1. Hum Mol Genet. 2006;15(13):2138–45. pmid:16723374.
  58. 58. Shcherbata HR, Yatsenko AS, Patterson L, Sood VD, Nudel U, Yaffe D, et al. Dissecting muscle and neuronal disorders in a Drosophila model of muscular dystrophy. EMBO J. 2007;26(2):481–93. pmid:17215867; PubMed Central PMCID: PMC1783456.
  59. 59. Ueyama M, Akimoto Y, Ichimiya T, Ueda R, Kawakami H, Aigaki T, et al. Increased apoptosis of myoblasts in Drosophila model for the Walker-Warburg syndrome. PLoS One. 2010;5(7):e11557. pmid:20644630; PubMed Central PMCID: PMC2903483.
  60. 60. Uchino R, Nonaka YK, Horigome T, Sugiyama S, Furukawa K. Loss of Drosophila A-type lamin C initially causes tendon abnormality including disintegration of cytoskeleton and nuclear lamina in muscular defects. Dev Biol. 2013;373(1):216–27. pmid:22982669.
  61. 61. Pantoja M, Ruohola-Baker H. Drosophila as a starting point for developing therapeutics for the rare disease Duchenne Muscular Dystrophy. Rare diseases. 2013;1:e24995. pmid:25002997; PubMed Central PMCID: PMC3932943.
  62. 62. Kucherenko MM, Pantoja M, Yatsenko AS, Shcherbata HR, Fischer KA, Maksymiv DV, et al. Genetic modifier screens reveal new components that interact with the Drosophila dystroglycan-dystrophin complex. PLoS One. 2008;3(6):e2418. pmid:18545683; PubMed Central PMCID: PMC2398783.
  63. 63. Garcia-Lopez A, Monferrer L, Garcia-Alcover I, Vicente-Crespo M, Alvarez-Abril MC, Artero RD. Genetic and chemical modifiers of a CUG toxicity model in Drosophila. PLoS One. 2008;3(2):e1595. pmid:18270582; PubMed Central PMCID: PMC2220037.
  64. 64. Brand AH, Perrimon N. Targeted gene expression as a means of altering cell fates and generating dominant phenotypes. Development. 1993;118(2):401–15. pmid:8223268.
  65. 65. Duffy JB. GAL4 system in Drosophila: a fly geneticist's Swiss army knife. Genesis. 2002;34(1–2):1–15. pmid:12324939.
  66. 66. Thummel C, Pirrotta V. New pCaSpeR P element vectors. Drosoph Inf Serv. 1992;71:150.
  67. 67. Iida T, Lilly MA. missing oocyte encodes a highly conserved nuclear protein required for the maintenance of the meiotic cycle and oocyte identity in Drosophila. Development. 2004;131(5):1029–39. pmid:14973288.
  68. 68. Blair SS. Drosophila Protocols. In: Sullivan W, Ashburner M, Hawley RS, editors.: Cold Spring Harbor Laboratory Press; 2000.
  69. 69. Morriss GR, Bryantsev AL, Chechenova M, LaBeau EM, Lovato TL, Ryan KM, et al. Analysis of skeletal muscle development in Drosophila. Methods Mol Biol. 2012;798:127–52. pmid:22130835.
  70. 70. Paro R. Drosophila Protocols. In: Sullivan W, Ashburner M, Hawley RS, editors.: Cold Spring Harbor Laboratory Press; 2000.
  71. 71. Kucherenko MM, Marrone AK, Rishko VM, Yatsenko AS, Klepzig A, Shcherbata HR. Paraffin-embedded and frozen sections of Drosophila adult muscles. Journal of visualized experiments: JoVE. 2010;(46). pmid:21206479; PubMed Central PMCID: PMC3159657.
  72. 72. Snider L, Asawachaicharn A, Tyler AE, Geng LN, Petek LM, Maves L, et al. RNA transcripts, miRNA-sized fragments and proteins produced from D4Z4 units: new candidates for the pathophysiology of facioscapulohumeral dystrophy. Hum Mol Genet. 2009;18(13):2414–30. Epub 2009/04/11. ddp180 [pii] pmid:19359275; PubMed Central PMCID: PMC2694690.
  73. 73. de la Kethulle de Ryhove L, Ansseau E, Nachtegael C, Pieters K, Vanderplanck C, Geens M, et al. The Role of D4Z4-Encoded Proteins in the Osteogenic Differentiation of Mesenchymal Stromal Cells Isolated from Bone Marrow. Stem cells and development. 2015. pmid:26192274.
  74. 74. Rorth P. Gal4 in the Drosophila female germline. Mech Dev. 1998;78(1–2):113–8. pmid:9858703.
  75. 75. Mitsuhashi H, Mitsuhashi S, Lynn-Jones T, Kawahara G, Kunkel LM. Expression of DUX4 in zebrafish development recapitulates facioscapulohumeral muscular dystrophy. Hum Mol Genet. 2013;22(3):568–77. pmid:23108159.
  76. 76. Lee T, Luo L. Mosaic analysis with a repressible cell marker for studies of gene function in neuronal morphogenesis. Neuron. 1999;22(3):451–61. pmid:10197526.
  77. 77. Seroude L, Brummel T, Kapahi P, Benzer S. Spatio-temporal analysis of gene expression during aging in Drosophila melanogaster. Aging cell. 2002;1(1):47–56. pmid:12882353.
  78. 78. Freeman M. Reiterative use of the EGF receptor triggers differentiation of all cell types in the Drosophila eye. Cell. 1996;87(4):651–60. pmid:8929534.
  79. 79. Thomas BJ, Wassarman DA. A fly's eye view of biology. Trends Genet. 1999;15(5):184–90. pmid:10322485.
  80. 80. Lee JH, Koh H, Kim M, Park J, Lee SY, Lee S, et al. JNK pathway mediates apoptotic cell death induced by tumor suppressor LKB1 in Drosophila. Cell death and differentiation. 2006;13(7):1110–22. pmid:16273080.
  81. 81. Jemc J, Rebay I. Targeting Drosophila eye development. Genome Biol. 2006;7(7):226. pmid:16879729; PubMed Central PMCID: PMC1779560.
  82. 82. Jemc J, Rebay I. Characterization of the split ends-like gene spenito reveals functional antagonism between SPOC family members during Drosophila eye development. Genetics. 2006;173(1):279–86. pmid:16547102; PubMed Central PMCID: PMC1461450.
  83. 83. Jin S, Martinek S, Joo WS, Wortman JR, Mirkovic N, Sali A, et al. Identification and characterization of a p53 homologue in Drosophila melanogaster. Proc Natl Acad Sci U S A. 2000;97(13):7301–6. pmid:10860994; PubMed Central PMCID: PMC16540.
  84. 84. Qing Y, Yin F, Wang W, Zheng Y, Guo P, Schozer F, et al. The Hippo effector Yorkie activates transcription by interacting with a histone methyltransferase complex through Ncoa6. eLife. 2014;3. pmid:25027438; PubMed Central PMCID: PMC4118621.
  85. 85. Moses K, Rubin GM. Glass encodes a site-specific DNA-binding protein that is regulated in response to positional signals in the developing Drosophila eye. Genes Dev. 1991;5(4):583–93. pmid:2010085.
  86. 86. Wernet MF, Labhart T, Baumann F, Mazzoni EO, Pichaud F, Desplan C. Homothorax switches function of Drosophila photoreceptors from color to polarized light sensors. Cell. 2003;115(3):267–79. pmid:14636555.
  87. 87. Li WZ, Li SL, Zheng HY, Zhang SP, Xue L. A broad expression profile of the GMR-GAL4 driver in Drosophila melanogaster. Genetics and molecular research: GMR. 2012;11(3):1997–2002. pmid:22911584.
  88. 88. Petrov A, Pirozhkova I, Carnac G, Laoudj D, Lipinski M, Vassetzky YS. Chromatin loop domain organization within the 4q35 locus in facioscapulohumeral dystrophy patients versus normal human myoblasts. Proc Natl Acad Sci U S A. 2006;103(18):6982–7. pmid:16632607.
  89. 89. Grewal PK, van Geel M, Frants RR, de Jong P, Hewitt JE. Recent amplification of the human FRG1 gene during primate evolution. Gene. 1999;227(1):79–88. pmid:9931447.
  90. 90. Hanel ML, Sun CY, Jones TI, Long SW, Zanotti S, Milner D, et al. Facioscapulohumeral muscular dystrophy (FSHD) region gene 1 (FRG1) is a dynamic nuclear and sarcomeric protein. Differentiation. 2011;81(2):107–18. Epub 2010/10/26. S0301-4681(10)00281-1 [pii] pmid:20970242; PubMed Central PMCID: PMC3030934.
  91. 91. Sun C-YJ, van Koningsbruggen S, Long SW, Straasheijm K, Klooster R, Jones TI, et al. FSHD region gene 1 (FRG1) is a dynamic RNA-associated actin bundling protein. J Mol Biol. 2011;In press.
  92. 92. Ferri G, Huichalaf CH, Caccia R, Gabellini D. Direct Interplay Between Two Candidate Genes in FSHD Muscular Dystrophy. Hum Mol Genet. 2014. pmid:25326393.
  93. 93. Nahabedian JF, Qadota H, Stirman JN, Lu H, Benian GM. Bending amplitude—a new quantitative assay of C. elegans locomotion: identification of phenotypes for mutants in genes encoding muscle focal adhesion components. Methods. 2012;56(1):95–102. Epub 2011/12/01. S1046-2023(11)00237-4 [pii] pmid:22126736; PubMed Central PMCID: PMC3299906.
  94. 94. Krom YD, Thijssen PE, Young JM, den Hamer B, Balog J, Yao Z, et al. Intrinsic Epigenetic Regulation of the D4Z4 Macrosatellite Repeat in a Transgenic Mouse Model for FSHD. PLoS Genet. 2013;9(4):e1003415. pmid:23593020.
  95. 95. Clapp J, Mitchell LM, Bolland DJ, Fantes J, Corcoran AE, Scotting PJ, et al. Evolutionary conservation of a coding function for D4Z4, the tandem DNA repeat mutated in facioscapulohumeral muscular dystrophy. Am J Hum Genet. 2007;81(2):264–79. Epub 2007/08/02. S0002-9297(07)61193-8 [pii] pmid:17668377.
  96. 96. Leidenroth A, Clapp J, Mitchell LM, Coneyworth D, Dearden FL, Iannuzzi L, et al. Evolution of DUX gene macrosatellites in placental mammals. Chromosoma. 2012;121(5):489–97. pmid:22903800.
  97. 97. Ferreboeuf M, Mariot V, Bessieres B, Vasiljevic A, Attie-Bitach T, Collardeau S, et al. DUX4 and DUX4 downstream target genes are expressed in fetal FSHD muscles. Hum Mol Genet. 2013. pmid:23966205.
  98. 98. Broucqsault N, Morere J, Gaillard MC, Dumonceaux J, Torrents J, Salort-Campana E, et al. Dysregulation of 4q35- and muscle-specific genes in fetuses with a short D4Z4 array linked to Facio-Scapulo-Humeral Dystrophy. Hum Mol Genet. 2013;22(20):4206–14. pmid:23777630.
  99. 99. Dandapat A, Bosnakovski D, Hartweck LM, Arpke RW, Baltgalvis KA, Vang D, et al. Dominant Lethal Pathologies in Male Mice Engineered to Contain an X-Linked DUX4 Transgene. Cell reports. 2014;8(5):1484–96. pmid:25176645.
  100. 100. Sharma V, Harafuji N, Belayew A, Chen YW. DUX4 Differentially Regulates Transcriptomes of Human Rhabdomyosarcoma and Mouse C2C12 Cells. PLoS One. 2013;8(5):e64691. pmid:23717650; PubMed Central PMCID: PMC3661531.
  101. 101. Himeda CL, Debarnot C, Homma S, Beermann ML, Miller JB, Jones PL, et al. Myogenic enhancers regulate expression of the facioscapulohumeral muscular dystrophy associated DUX4 gene. Mol Cell Biol. 2014;34(11):1942–55. pmid:24636994; PubMed Central PMCID: PMC4019064.
  102. 102. Picchio L, Plantie E, Renaud Y, Poovthumkadavil P, Jagla K. Novel Drosophila model of myotonic dystrophy type 1: phenotypic characterization and genome-wide view of altered gene expression. Hum Mol Genet. 2013;22(14):2795–810. pmid:23525904.
  103. 103. Haines N, Seabrooke S, Stewart BA. Dystroglycan and protein O-mannosyltransferases 1 and 2 are required to maintain integrity of Drosophila larval muscles. Mol Biol Cell. 2007;18(12):4721–30. pmid:17881734; PubMed Central PMCID: PMC2096576.
  104. 104. Wairkar YP, Fradkin LG, Noordermeer JN, DiAntonio A. Synaptic defects in a Drosophila model of congenital muscular dystrophy. The Journal of neuroscience: the official journal of the Society for Neuroscience. 2008;28(14):3781–9. pmid:18385336.
  105. 105. Dialynas G, Speese S, Budnik V, Geyer PK, Wallrath LL. The role of Drosophila Lamin C in muscle function and gene expression. Development. 2010;137(18):3067–77. pmid:20702563; PubMed Central PMCID: PMC2926956.