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Logo of nihpaAbout Author manuscriptsSubmit a manuscriptNIH Public Access; Author Manuscript; Accepted for publication in peer reviewed journal;
Nature. Author manuscript; available in PMC May 20, 2009.
Published in final edited form as:
PMCID: PMC2597674
NIHMSID: NIHMS67900

The zinc-finger protein Zelda is a key activator of the early zygotic genome in Drosophila

Abstract

In all animals, the initial events of embryogenesis are controlled by maternal gene products that are deposited into the developing oocyte. At some point after fertilization, control of embryogenesis is transferred to the zygotic genome in a process called the maternal to zygotic transition (MZT). During this time many maternal RNAs are degraded and transcription of zygotic RNAs ensues1. A longstanding question has been, what factors regulate these events? The recent findings that microRNAs2,3 and Smaugs4 mediate maternal transcript degradation have shed new light on this aspect of the problem. However, the transcription factor(s) that activate the zygotic genome remain elusive. The discovery that many of the early transcribed genes in Drosophila share a cis-regulatory heptamer motif, CAGGTAG and related sequences5,6, collectively referred to as TAGteam sites5 brought up the possibility that a dedicated transcription factor could interact with these sites to activate transcription. Here we report that the zinc-finger protein, Zelda (Zld; Zinc-finger early Drosophila activator), binds specifically to these sites, and is capable of activating transcription in transient transfection assays. Mutant embryos lacking zld are defective in cellular blastoderm formation, and fail to activate many genes essential for cellularization, sex determination, and pattern formation. Global expression profiling confirmed that Zld plays a key role in the activation of the early zygotic genome, and suggests that Zld may also regulate maternal RNA degradation during the MZT.

In Drosophila, an initial wave of zygotic gene transcription occurs between 1-2 hours of development during mitotic cleavage cycles 8-13. This is followed by a major burst of activity between 2-3 hours (cycle 14) when the embryo is undergoing cellular blastoderm formation. Many pre-cellular genes contain TAGteam sites in their upstream regulatory regions including several direct targets of Bicoid, Dorsal, and other key regulators of patterning5-7. ten Bosch et. al.5 demonstrated that TAGteam sites are required for the early expression of the dorsoventral (DV) gene zen, and the sex determination genes sisB and Sxl. To isolate the TAGteam binding factor, we performed a yeast one-hybrid screen with a 91 bp fragment (Fig. 1a, sequences in uppercase) from the zen cis-regulatory region8,9, which contains four TAGteam sites5 (Fig. 1a in red, the first two are the reverse complement). zld (CG12701 on the X-chromosome) was selected as the only candidate of the 11 recovered that had the potential to bind specific DNA sequences since it encoded a protein with six C2H2 zinc fingers (represented as green boxes in Fig. 1b). Oligonucleotides (Fig. 1a, underlined sequences) with different TAGteam sites were tested in gel shift assays with the 357 amino-acid C-terminal region of Zld fused to GST (GST-ZldC; Fig. 1b, stippled region). They all formed complexes with GST-ZldC, though with different affinities (Fig. 1c lanes 1-9), while mutations (Fig. 1a, in purple) in the heptanucleotide sequence abolished binding (Fig. 1c, lanes 10-12). Interestingly, the site with the strongest affinity, CAGGTAG, is the site most over represented in regulatory elements of pre-blastoderm genes versus postblastoderm genes5. A plasmid expressing full-length Zld protein promoted transcriptional activation of a zen91-lacZ reporter but not a mutated zen91m-lacZ reporter after co-transfection in Drosophila S2 cells (Fig. 1d). Taken together, these data strongly suggest that Zld activates transcription of zen, and likely other TAGteam containing genes.

Figure 1
TAGteam sites bind Zld and mediate transcriptional activation

zld transcripts were detected in the germline cells of the ovary (Fig. 2a), in unfertilized eggs (Fig. 2b), and throughout early development (Fig. 2c). Later zld becomes restricted to the nervous system and specific head regions (Fig. 2d), as previously shown10. To analyze zld function, we generated deletion alleles of zld by imprecise excision (schematized in Fig. 1b). Hemizygous embryos showed abnormal CNS and head development (data not shown), consistent with previous reports of CG12701 lethal P-insertion phenotypes10,11. zld transcripts were not observed in these embryos after cycle 14 (Fig. 2e). However, younger embryos had high levels of maternal zld transcripts (data not shown), indicating that maternally loaded zld transcripts are degraded during cellularization, and replaced with zygotic zld.

Figure 2
Maternal zld transcripts are lost as zygotic zld is activated in cycle 14

To eliminate maternal zld from embryos, we induced clones of zld294 mutant germ cells in the adult female. All resulting embryos were null for maternal zld (M- zld), and the male embryos were also null for zygotic zld (M-Z- zld). All early M- zld embryos lacked zld transcripts (Fig. 2f), but had normal patterns of other maternally deposited factors such as bicoid RNAs (Fig. 2g) and the Dorsal protein gradient (data not shown). M-Z- zld embryos never expressed zld (Fig. 2h) unlike M-Z+ zld embryos, which began to express zld ubiquitously in cycle 14 (Fig. 2i). However, regardless of their zygotic genotypes, all M- zld embryos showed a severe abnormal morphology after cycle 14 (Fig. 2h,j), and did not survive to make cuticle.

Before cycle 14, M zld embryos are similar to wild-type, except for sporadic nuclear fallout (Fig. 3c’). However, at early cycle 14 the hexagonal-actin network becomes disorganized (Fig. 3c) and begins to degenerate (Fig. 3d) resulting in a multinucleated phenotype (Fig. 3d”, arrow) resembling nullo12 and serendipity-α13 (sry-α) mutants. Celllarization does not proceed as furrow canals never move inward (Fig. 3d, arrow) like in wild-type (Fig. 3b, arrow), and Neurotactin (Nrt) accumulates abnormally in the apical cytoplasm (Fig. 3h, arrow), reminiscent of the slam mutant phenotype14,15. Staining with α-Slam antibody confirmed that Slam protein is mostly absent by mid-cycle 14 (Fig. 3f) while in wild-type, Slam has moved basally (Fig. 3e’). In addition, nuclei do not elongate but instead become rounded, enlarged, and clump together (Fig. 3f and h’ arrow). Regions of higher nuclear density were observed (data not shown), a phenotype similar to that obtained by injection of dsRNA against CG1270110, which we noticed resembles a frühstart (frs) phenotype16. Despite their aberrant morphology, M- zld embryos attempt to form a ventral furrow (Fig. S1b,c,e) but soon become highly disorganized with only pole cells recognizable (Fig. S1f). We rescued the M- zld cellularization defects by driving a wild-type copy of zld in the germline using the ovarian tumor (otu) promoter17. The cytoskeleton becomes well structured (Fig. 3i) and furrow canal ingression are normal (Fig. 3i’) as Slam protein is restored (data not shown).

Figure 3
Maternal zld is required for cellularization

The broad range of phenotypes strongly indicated that M- zld embryos do not express genes essential for cellular blastoderm formation. We assayed the expression of sry-α, slam, and nullo, as well as sisA, sisB, sisC, Sxl, zen and dpp. None of these genes were activated in M- zld embryos (data shown for sry-α, sisB , and zen in Fig. 4b, d, f, respectively), except at the poles in some cases. However, sna and sog, which are activated by Dorsal18, were not absent but delayed in expression by at least 2 cycles (data not shown), suggesting that Zld facilitates the onset of early-gene transcription. Furthermore, the lateral stripes of sog were greatly reduced in width (Fig. 4h), indicating that in regions where Dorsal protein levels are low, a combinatorial mechanism involving both Dorsal and Zld establishes the broad sog domain. Interestingly, the two TAGteam sites in the 393bp sog enhancer19 lie close to four Dorsal binding sites.

Figure 4
Zld plays a role in zygotic gene activation and maternal RNA degradation during the MZT

Our results hinted that Zld is a global activator of early genes. To test this directly we compared the expression profiles of wild-type and M- zld embryos in mitotic cycles 8-13, a time point presumably enriched in genes that are direct Zld targets. 120 genes were down-regulated at least 2-fold, and surprisingly 176 genes were up-regulated, in the absence of Zld (p<0.05; Fig. 4k). The down-regulated set (Table S1) was strongly enriched in genes that are zygotically expressed (Fig. 4l) and involved in early developmental processes (Fig. S2), including most of the genes we assayed by in situ (Fig. 4k). For example, 12 genes involved in cellular blastoderm formation (nullo, slam, sry-α, bnk, frs, btsz, halo and 5 halo-like genes20), 6 sex determination genes (sisA, sisB, sisC, run, Sxl, dpn), and 8 DV genes (dpp, tld, tok, tsg, tsg-like, scw, zen, zen-2) are in our down-regulated dataset. Overall, 75% of the early genes previously described as pre-cellular5,6,21 are included. This number may be an underestimate since there may be many genes like sna and sog that did not make the 2-fold cut-off (Fig. 4k), but are indeed regulated by Zld.

About 80% of the down-regulated genes have TAGteam sites within 2 Kb upstream of the transcription start site (Table S2), and another 10% have TAGteam sites in introns, such as slam with two sites in its first intron, supporting the idea that most of our down-regulated genes are direct Zld targets. In addition, the TAGteam sites upstream of the down-regulated genes tend to be located very close to the transcription start site, within 200 bp (Table S2), consistent with the previous finding that early zygotic genes have a statistical overrepresentation of TAGteam sites close to the start site5,6.

In contrast to the down-regulated genes, the up-regulated set is strongly enriched in genes that are maternally expressed (Fig. 4l). We considered the possibility that Zld activates components of the RNA degradation machinery that in turn destabilize maternal RNAs. Since the miR-309 enhancer22 contains two TAGteam sites, we assayed for miR-309 primary transcripts in M- zld embryos (Fig. 4j), and indeed they were absent. It was recently shown that mature miR-309 miRs become abundant during cycle 14, and play a role in maternal transcript turnover in 2-4 hr embryos3. Not surprisingly, our 1-2 hr (cycles 8-13) dataset had no overlap with the 44 published miR-309 targets3, however 2-4 hr profiling experiments should reveal whether they are up-regulated in the absence of zld. We also compared our up-regulated genes to those affected by smaug4, another gene required for removal of maternally supplied RNAs. We found there was little overlap with the published Smaug targets4, suggesting that Zld is involved in a parallel pathway of maternal RNA degradation.

In summary, we have demonstrated that Zld functions as a key transcriptional activator during the MZT in Drosophila. This is the first demonstration of such an activator in any organism. We propose that the biological role of Zld in the preblastoderm embryo is to set the stage for key processes such as cellular blastoderm formation, counting of X chromosomes for dosage compensation and sex determination, and pattern formation, by ensuring the coordinated accumulation of batteries of gene products during the MZT. This early preparedness should allow sufficient time for the formation of molecular machines23 involved in these processes, and so are ready to spring into action during the prolonged interphase of cycle 14.

Methods Summary

Fly strains

The zld294 and zld681 alleles were generated by imprecise excision of the P{RS3}24 element UM-8171-3 (Flybase, Szeged stock center). The ovoD FRT19A stock was generated by transposition of P{mini w+, ovoD1-26}25 onto y w sn FRT19A, hsFLP122. Germ-line clones were induced in zld294 FRT 19A / ovoD1 FLP122 FRT19A by the Flp-FRT technique26. Virgin females were collected and mated to yw, FM7, or FM7c-ftz-lacZ males. The otu-zld construct was microinjected into w1118 embryos.

Yeast one-hybrid assay

The yeast one-hybrid screen was performed following the Matchmaker One-Hybrid System (Clontech) protocol with the 91 bp zen-promoter and a 0-6 hours Drosophila embryonic cDNA library fused to the Gal4 activation domain27 (gift from L. Pick).

Molecular Biology

DNA binding assays9 and Drosophila S2 cell transient transfection assays28 were performed as previously described. The fold activation was calculated as a ratio of the normalized (for transfection efficiency) lacZ activity in cells treated with 0.5 mM CuSO4 and untreated cells.

Analysis of phenotypes

Various RNA probes, antibodies and molecular probes were used to detect gene expression or to visualize the cytoskeleton and nuclei (further described in the online Methods). Embryos were viewed by fluorescence microscopy using a Nikon FX-A microscope for whole embryo views, or an Improvision Yokogawa CSU-10 spinning disk confocal system for grazing and sectional views, and by Nomarski optics using a Zeiss Axiophot microscope.

Microarray analysis

Total RNA was extracted from three independent collections of 1-2 hr yw and M- zld embryos by TRIzol (invitrogen). cDNA was prepared using the GeneChip® HT One-Cycle cDNA Synthesis Kit (Invitrogen), labeled with the BioArray™ HighYield™ RNA Transcript Labeling Kit (Enzo), and hybridized to Affymetrix Drosophila Genome 2 arrays and processed by a GeneChip Fluidics Station 400.

Supplementary Material

Acknowledgements

We thank the following people for generous gifts of RNA probes, plasmids, antibodies, and fly stocks: J. Erickson, R. Lehmann, R. Cinalli, R. Martinho, C. Navarro,J. Treisman, and L. Pick. We are indebted to J. Rhee, and A. Chung for help with isolating and characterizing zld null mutants. We thank S. Fu for help locating TAGteam sites in Zelda target genes. We are grateful to M. Siegel and K. Birnbaum for help with the microarray analysis, and C. Desplan, P. Struffi, S. Small, and R. Lehmann for critical reading of the manuscript. This work was supported by a grant from the National Institutes of Health (GM63024).

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