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First published online December 7, 2007
doi: 10.1242/10.1242/dev.009050

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Insertional mutagenesis by the Tol2 transposon-mediated enhancer trap approach generated mutations in two developmental genes: tcf7 and synembryn-like

Saori Nagayoshi¹, Eriko Hayashi², Gembu Abe¹, Naoki Osato³, Kazuhide Asakawa¹, Akihiro Urasaki¹, Kazuki Horikawa^2,*, Kazuho Ikeo^3,4, Hiroyuki Takeda² and Koichi Kawakami^1,4,

¹ Division of Molecular and Developmental Biology, National Institute of Genetics, Mishima, Shizuoka 411-8540, Japan.
² Department of Biological Sciences, University of Tokyo, Tokyo 113-0033, Japan.
³ Center for Information Biology and DNA Data Bank of Japan, National Institute of Genetics, Mishima, Shizuoka 411-8540, Japan.
⁴ Department of Genetics, The Graduate University of Advanced Studies (SOKENDAI), Mishima, Shizuoka 411-8540, Japan.

Author for correspondence (e-mail: kokawaka{at}lab.nig.ac.jp)

Accepted 19 October 2007

	SUMMARY

TOP SUMMARY INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

 
Gene trap and enhancer trap methods using transposon or retrovirus have been recently described in zebrafish. However, insertional mutants using these methods have not been reported. We report here development of an enhancer trap method by using the Tol2 transposable element and identification and characterization of insertional mutants. We created 73 fish lines that carried single copy insertions of an enhancer trap construct, which contained the zebrafish hsp70 promoter and the GFP gene, in their genome and expressed GFP in specific cells, tissues and organs, indicating that the hsp70 promoter is highly capable of responding to chromosomal enhancers. First, we analyzed genomic DNA surrounding these insertions. Fifty-one of them were mapped onto the current version of the genomic sequence and 43% (22/51) were located within transcribed regions, either exons or introns. Then, we crossed heterozygous fish carrying the same insertions and identified two insertions that caused recessive mutant phenotypes. One disrupted the tcf7 gene, which encodes a transcription factor of the Tcf/Lef family mediating Wnt signaling, and caused shorter and wavy median fin folds and pectoral fins. We knocked down Lef1, another member of the Tcf/Lef family also expressed in the fin bud, in the tcf7 mutant, and revealed functional redundancy of these factors and their essential role in establishment of the apical ectodermal ridge (AER). The other disrupted the synembryn-like gene (synbl), a homolog of the C. elegans synembryn gene, and caused embryonic lethality and small pigment spots. The pigment phenotype was rescued by application of forskolin, an activator of adenylyl cyclase, suggesting that the synbl gene activates the G_S pathway leading to activation of adenylyl cyclase. We thus demonstrated that the transposon-mediated enhancer trap approach can indeed create insertional mutations in developmental genes. Our present study provides a basis for the development of efficient transposon-mediated insertional mutagenesis in a vertebrate.

Key words: Zebrafish, tcf7, synembryn, Enhancer trapping, Insertional mutagenesis

	INTRODUCTION

TOP SUMMARY INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

 
In zebrafish, phenotype-driven mutagenesis screens have been performed by two ways. First, chemical mutagenesis screens using ENU have identified hundreds of mutations that cause defects in various processes of embryonic development (Driever et al., 1996; Haffter et al., 1996). Identification of genes responsible for the mutant phenotypes requires positional cloning, which is still laborious (although sequencing and annotation of the genome are nearing completion). Second, a pseudotyped retrovirus has been used to mutagenize the genome (Gaiano et al., 1996). By using this approach, more than 300 recessive lethal mutants and the mutated genes have been identified (Amsterdam et al., 2004). However, a large-scale insertional mutagenesis screen using pseudotyped retrovirus is demanding in terms of labor and space because it requires raising of a large number of F2 families to identify mutant phenotypes in F3 embryos (Amsterdam et al., 1999).

Recently, gene trap and enhancer trap methods were developed in zebrafish. In gene trapping, a Tol2 transposon construct containing a splice acceptor and the GFP gene was constructed. When the construct was integrated within a gene and the splice acceptor trapped its transcript, GFP is expressed (Kawakami et al., 2004). In enhancer trapping, a Sleeping Beauty construct containing a modified EF1 promoter and the GFP gene (Balciunas et al., 2004), a Tol2 construct containing the keratin8 promoter and the GFP gene (Parinov et al., 2004), and a retroviral construct containing the gata2 promoter and the YFP gene (Ellingsen et al., 2005) were used. When the enhancer trap constructs were integrated in the genome and the minimal promoters were activated by enhancers, GFP or YFP is expressed in regulated fashions. It has been demonstrated that these methods can create transgenic fish expressing the reporter proteins in specific cells, tissues and organs, which are useful resources for developmental biology. However, it has not been reported that insertions of these gene trap or enhancer trap constructs can cause any observable mutant phenotype.

We found that the medaka fish Tol2 element encodes a fully functional transposase (Kawakami et al., 1998; Kawakami and Shima, 1999; Kawakami et al., 2000) and, since then, have been developing genetic methods in zebrafish by using Tol2 (Kawakami, 2005). Our goal is to develop an efficient transposon-mediated insertional mutagenesis method as follows. First, random integrations of a gene trap or an enhancer trap construct are created in the genome of the germ cells in the fish (F0) injected with a transposon-donor plasmid and the transposase mRNA. Second, F1 embryos exhibiting unique GFP expression patterns are collected and raised. Third, by mating male and female F1 fish that carry the same insertion, F2 embryos are analyzed for the mutant phenotype. If an insertion disrupted an essential gene, homozygous embryos show a mutant phenotype. Finally, the gene responsible for the mutant phenotype can be cloned rapidly, as the locus is tagged by the transposon. Zebrafish researchers should benefit from this methodology because it will require maintenance of smaller numbers of F1 fish than chemical mutagenesis or retroviral mutagenesis, and the F2 screen will be carried out within a shorter period of time than the F3 screen.

As a first step toward this goal, it is important to demonstrate that a transposon-mediated gene trap or enhancer trap method can indeed create a mutant. In our previous gene trap screen, we created homozygous embryos by mating, but could not identify recessive phenotypes (Kawakami et al., 2004; Kotani et al., 2006). In addition, in the previous gene trap and enhancer trap screens using transposons and retrovirus, recessive mutant phenotypes have not been analyzed extensively (Balciunas et al., 2004; Ellingsen et al., 2005; Parinov et al., 2004). In the present study, we constructed an enhancer trap construct containing the zebrafish hsp70 promoter and the GFP gene, performed an enhancer trap screen, and established fish lines expressing GFP in specific cells and tissues. We then analyzed phenotypes of homozygous embryos by crossing these lines and found that insertions in the tcf7 and the synembryn-like (synbl) gene caused recessive mutant phenotypes. Tcf7 is a transcription factor mediating Wnt signaling. Although the zebrafish tcf7 gene was cloned previously (Veien et al., 2005), no mutation has been reported. synbl is a zebrafish homolog of the C. elegans synembryn gene, the product of which has been shown to activate both the G_q and G_S pathway, leading to production of diacylglycerol and cyclic AMP, respectively (Miller et al., 2000; Schade et al., 2005). Previously, a mutation of synbl was identified by retroviral insertional mutagenesis (Amsterdam et al., 2004), but its phenotype has not been characterized in detail. We will describe characterization of these mutants and demonstrate that insertions of the enhancer trap construct can indeed disrupt the function of developmental genes.

	MATERIALS AND METHODS

TOP SUMMARY INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

 
Construction of T2KHG transgenic fish
T2KHG contains the hsp70 promoter (a kind gift from Dr J. Kuwada) (Halloran et al., 2000), the GFP gene and the polyA signal between Tol2 cis-sequences (Urasaki et al., 2006) (see Fig. 3A). A DNA/RNA mixture (1 nl) containing 30 ng/µl plasmid DNA harboring T2KHG and 5 ng/µl transposase mRNA synthesized in vitro was injected into fertilized eggs. F1 fish were analyzed under a fluorescent microscope MZ 16 FA (Leica).

Computational analyses
The integration sites were mapped on the zebrafish genome sequence (Zv6) by BLAT (Kent, 2002). Fifty-one random insertions were created 10,000 times by using the computer system in DDBJ, NIG. The locations of mRNA and Ensemble transcripts were obtained from all_mrna.txt.gz and ensGene.txt.gz (http://hgdownload.cse.ucsc.edu/goldenPath/danRer4/database/), and analyzed by using in-house Perl scripts. RIC8A and RIC8B were aligned by CLUSTAL W (Thompson et al., 1994), and the phylogenetic tree was constructed by the neighbor-joining method (Saitou and Nei, 1987) and the minimum evolution method (Rzhetsky and Nei, 1992) with p-distance. Each node of the phylogenetic tree was evaluated by 1000 bootstrap replications (Felsenstein, 1985).

Whole-mount in situ hybridization
Probes were synthesized with DIG RNA labeling kit (Roche), and purified with mini Quick Spin RNA Columns (Roche). Prehybridization and hybridization were performed at 65°C for 1 hour to over night. The samples were washed in 66% formamide/2xSSCT at 65°C for 30 minutes, in 33% formamide/2xSSCT at 65°C for 30 minutes, in 2xSSCT at 65°C for 15 minutes, and in 0.2xSSCT at 65°C for 30 minutes twice. The samples were then incubated in blocking solution (150 mM maleic acid, 100 mM NaCl, 5% blocking reagent (Roche), 5% new born calf serum, pH 7.5, 0.1% Tween-20) at 4°C overnight, then incubated with 1/4000-1/8000 volume of anti-digoxigenin-AP Fab-fragments (Roche) at room temperature for 4 hours or at 4°C overnight. Samples were washed in maleic acid buffer (150 mM maleic acid, 100 mM NaCl, 0.1% Tween-20, pH 7.5) at room temperatures for 25 minutes three times and then overnight. The signals were detected by using BCIP/NBT Color Development Substrate (Promega). The reaction was stopped by washing with PBS.

Southern blot hybridization and PCR analyses
Southern blot hybridization, inverse PCR, linker-mediated PCR, RT-PCR, 3' RACE and 5' RACE were carried out as described previously (Kawakami, 2004; Kotani et al., 2006). Primers used for these analyses are as follows.

HG2A: 5'-GAG GAG AAG AAG GGC CAT CTC ATT C-3' (forward) and 5'-CTA CAT AAC ACT CTC GAA AAT GAT C-3' (reverse)

HG3A: 5'-GTC CTG AAC TCA ATC TGT CAT C-3' (forward) and 5'-CTG AGT TAC CTG AGA ACT GTG A-3' (reverse)

HG6A: 5'-TCC AGC ACT GAA GTA TGC AGA AAT G-3' (forward) and 5'-TCA CAG TTT GGC AGC CAT GAA G-3' (reverse)

HG6B: 5'-ATG TCT TCC AAG CAA GCC ACC TC-3' (forward) and 5'-GTG TCA TTC TCA CTG CTG TAG TCC-3' (reverse)

HG6C: 5'-AGT CGG TTT TAT GTT GTC GGA AAA G-3' (forward) and 5'-TCT GTA GGA TGA GTA GAG CGA-3' (reverse)

HG6D: 5'-AGC CGT GAG TCT GTT CAG CTG C-3' (forward) and 5'-CCT TGC CAT CAC AGA TGC CGT T-3' (reverse)

HG10A: 5'-CAG CGA TTG ACT GTT TTC CGC AAC-3' (forward) and 5'-CTA CTC TGA ATG AAC AGA CTG TTG-3' (reverse)

HG21A: 5'-GCA GAT TGA ACT CAT CAC CAC TGC-3' (forward) and 5'-CAC TGA TCA GGC TTT TAT GCG AGT-3' (reverse)

HG21B: 5'-CAG TGT GAT CCC ACG AGC TCC TCC-3' (forward) and 5'-CTT CAG ATC TTC TAG TCC AGT AGA-3' (reverse)

HG21C: 5'-GAC GTC TTG AGA AAG TTT GGA T-3' (tcf7-f1) and 5'-GGT TTG TCA GGT GAT AGA CAG G-3' (reverse)

HGn8H: 5'-GTG CAG AAG GAC TGA CAG TGT T-3' (synbl-f) and 5'-CTC GAC GGC AGC TCA TTC TTC T-3' (synbl-r2)

HGn43A: 5'-GTT TGA CCT GGT GCA TTA CGA G-3' (forward) and 5'-TCA AGG GCT TTT CTG CTG GAG T-3' (reverse)

ric8a: 5'-GGA ACA GCG ATG AAA ATG GAC T-3' (forward) and 5'-GTG GGT TAA ATT AAG TCG AAC C-3' (reverse)

To prepare RNA from heat-shocked embryos, about ten 24 hpf embryos are placed at 40°C for 15 minutes in a microtube, and lysed in TRIzol reagent (Invitrogen) immediately after the heat-shock treatment.

MO injection
Antisense morpholino oligonucleotides (MO) (Gene Tools) against translation initiation sites of tcf7 (tcf7-MO) and lef1 (lef1-MO) and a splice donor of synbl (synbl-MO) were synthesized:

tcf7-f2: 5'-GTG TTT CCA AAC ATG TAT GAG T-3'

tcf7-r2: 5'-GAC TGT TTG TTA GTT TGA GGC T-3'

tcf7-f3: 5'-GAA CGA CGA GAT GAT CGC GTT T-3'

synbl-r: 5'-CTA CGA TCA CAA GGC AAA TAC C-3'

Tol2-OUT: 5'-AGG ACC AAT GAA CAT GTC TGA CCA A-3'

tcf7-r3: 5'-GGG ACT GGG GTT GAA GTG TTC A-3'

tcf7-MO: GCT GCG GCA TGA TCC AAA CTT TCT C

symbl-MO: ACT GTC ACT CTC ACC TTA TCA CAG G

lef1-MO: CTC CAC CTG ACA ACT GCG GCA TTT C

One-cell stage embryos were injected with 0.1-1 nl of 1-3 mg/ml MOs suspended in H₂O using FemtoJet (Eppendorf).

Pigmentation analysis and forskolin treatment
Embryos were placed in the dark for at least 30 minutes and then observed soon after they were transferred onto the stage of a microscope. One-cell stage embryos were soaked in 1 µM or 2 µM of forskolin (Calbiochem) dissolved in 1% DMSO. As a control, embryos were soaked in 1% DMSO.

	RESULTS

TOP SUMMARY INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

 
An enhancer trap screen using the Tol2 enhancer trap construct
We constructed T2KHG that contained the zebrafish hsp70 promoter and the EGFP gene (see Fig. 3A). We expected that transcription from the hsp70 promoter to be activated at normal temperatures when it was influenced by chromosomal enhancers. We co-injected transposon-donor plasmid DNA containing the T2KHG construct and the transposase mRNA, crossed 77 injected fish with wild-type fish, and analyzed at least 40 embryos from each cross for GFP expression. We found that offspring (F1) from 70% (54/77) of the injected fish carried T2KHG insertions and showed more than 100 different GFP expression patterns. The GFP-positive F1 fish were raised and analyzed by Southern blot hybridization. The number of transposon insertions carried by individual F1 fish varied, from one to more than ten. Excluding fish with more than ten insertions, we analyzed 276 F1 fish and detected 215 different transposon insertions. These fish were further outcrossed to establish fish lines with single insertions. In the course of the outcross, we observed a total of 125 unique GFP expression patterns (Table 1).

We cloned and sequenced genomic DNA surrounding the 73 insertions. Fifty-one insertions were successfully mapped by BLAT against the zebrafish genome (Zv6) (see Table S1 in the supplementary material). First, these sequences were subjected to a computational analysis to determine whether the insertions were located within transcribed regions. Thirty-three percent of them (17/51) were localized within transcribed regions defined based on mRNA (all_mrna.txt.gz) and Ensembl (ensGene.txt.gz) transcripts. It was estimated by a computational analysis that, if transposon hit the zebrafish genome at random, 37.5% of the insertions would be located within the transcribed regions, indicating that the observed and the estimated frequencies are not statistically different. By comparison, we performed a similar computational analysis on previously reported 92 integration sites created by a retroviral enhancer trap construct (Ellingsen et al., 2005). Fifty one of them were mapped on the genome and 23.5% (12/51) were located within the transcribed region. With statistical significance, this frequency is lower than that observed in our present screen (P<0.05). The frequency calculated for the retroviral enhancer trapping is lower than the previous estimate (41%) (Ellingsen et al., 2005) as we used more stringent criteria for transcribed regions here.

Expression patterns of genes at the integration sites
To compare the GFP expression patterns with expression patterns of the genes at the integration sites, we performed RT-PCR for eight genes identified in HG3A, HG6C, HG6D, HG10A, HG10B HG21C, HGn8H and HGn43A. In all of these cases, cDNA clones were successfully obtained, indicating that the genes were indeed transcribed. Furthermore, we performed RT-PCR for eight genes found at the integration sites in HG2A, HG6A, HG6B, HG21A, HG21B, HG21K, HGn15B and HGn54A, which are predicted genes based on either EST, GenScan or Nscan, but not are the mRNA or Ensembl transcripts. In five cases (HG2A, HG6A, HG6B, HG21A, and HG21B), RT-PCR products were amplified, indicating that these were transcribed. Taking these into account, 43% (22/51) of the insertions were localized within protein-coding transcribed genes (Table 1) (see Table S1 in the supplementary material).

Then, we performed whole-mount in situ hybridization using the chot1 (HG2A), cyp2e2 (HG3A), ide (HG6A), soxlz (HG6B), uros (HG6C), asb1 (HG6D), ripk2 (HG10B), lmo7 (HG21A), hg21b (novel gene; HG21B), tcf7 (HG21C) and synbl (HGn8H) probes. Expression of chot1 (myotome; Fig. 2A,B), cyp2e2 (yolk; Fig. 2C,D), ide (myotome, Fig. 2E,F), soxlz (myotome; Fig. 2G,H), uros (ventral mesoderm; Fig. 2I,J), lmo7 (myotome; Fig. 2K,L), hg21b (otic vesicle; Fig. 2M,N), and tcf7 (median fin fold; Fig. 3B,C) recapitulated respective GFP expression patterns, at least partly, indicating that the hsp70 promoter was activated by enhancers that regulated those genes. By contrast, asb1 (HG6D), synbl (HGn8H) and ripk2 (HG10B) were expressed weakly in the whole body (data not shown). These were not similar to the GFP expression patterns. In these cases, the hsp70 promoter was likely to be influenced by enhancers that regulate expression of their neighboring genes. We will describe such an example in the case of HGn8H below.

The HG21C insertion disrupted the tcf7 gene
To elucidate whether the T2KHG insertions can cause observable mutant phenotypes, we analyzed phenotypes of homozygous embryos for 54 insertions including 20 insertions mapped within transcribed regions (see Table S1 in the supplementary material). We found morphological defects in the progeny from HG21C and HGn8H heterozygous parents.

In HG21C, T2KHG was integrated within the tcf7 gene that encodes a transcription factor downstream of Wnt signaling (Fig. 3A, Fig. 5A). GFP fluorescence and gfp mRNA were detected in the dorsal retina, diencephalon, tail bud and median fin fold at 24 hpf (Fig. 1, Fig. 3B). Although tcf7 mRNA was detected in broad areas in the brain, gfp mRNA did not show such an expression pattern (Fig. 3B,C), suggesting that a putative brain enhancer of tcf7 did not influence the hsp70 promoter. We analyzed 568 embryos obtained from HG21C heterozygous parents (Fig. 3D-H). One hundred and fifty-four out of 420 GFP-positives, but none of 148 GFP-negatives, showed short and wavy median fin folds at 60-72 hpf. Then, we performed genotyping by PCR and found that all of 83 GFP-positives with the fin phenotype were homozygous and all of 139 GFP-positives without the fin phenotype were heterozygous (Fig. 3I,J). These results strongly suggested that the observed fin defect is a recessive mutant phenotype caused by the transposon insertion. The length of the median fins was restored to nearly the wild-type level after day 6, but the wavy edge was observed at least until day 14 (data not shown). The homozygous fish were viable and fertile.

View larger version (113K): [in this window] [in a new window]   Fig. 1. GFP expression patterns in enhancer trap lines. GFP expression patterns in 24 hpf to day 5 embryos carrying single T2KHG insertions. Numbers after HG represent individual founder fish. Letters after numbers represent distinct patterns obtained from single founder fish. The patterns and transposon integration sites are described in Table S1 in the supplementary material.

View larger version (64K): [in this window] [in a new window]   Fig. 2. Expression patterns of genes at the integration sites. (A,C,E,G,I,K,M) Whole-mount in situ hybridization of embryos heterozygous for respective insertions (bottom right) at 24 hpf using the gfp probe. (B,D,F,H,J,L,N) Whole-mount in situ hybridization of wild-type embryos at 24 hpf using probes indicated (top right). Signals were detected in myotome (A,B), yolk (C,D), myotome (E-H), ventral mesoderm (I,J), myotome (K,L) and otic vesicle (M,N).

We then analyzed expression of tcf7 and lef1 in the pectoral fin bud at the AER induction (28 hpf) and maintenance (38 hpf) stages. The tcf7 expression was detected strongly in the AER and weakly in the mesenchyme at 28 hpf and 36 hpf (Fig. 4D,F), while the lef1 expression was detected both in the AER and mesenchyme at 28 hpf and only in the mesenchyme at 36 hpf (Fig. 4E,G). The unique expression of tcf7 in the AER at 36 hpf may account for the small and wavy fin phenotype observed in the HG21C homozygous embryos at later stages (Fig. 3S,T). To define the defects in lef1 and tcf7 loss-of-function embryos, we analyzed expression of mesenchymal (fgf10) and ectodermal (dlx2a, fgf24, wnt3l and fgf8) markers (Akimenko et al., 1994; Fischer et al., 2003; Norton et al., 2005; Reifers et al., 1998) in the lef1-MO-injected embryos. At 28 hpf, the mesenchymal fgf10 expression was similar in lef1-MO-injected wild-type and tcf7 mutant embryos (Fig. 4H,I). By contrast, expression of dlx2a in the AER was severely reduced in the lef1-MO-injected tcf7 mutant embryos; i.e. the expression was absent in about half of the injected embryos and detectable but very weak in the rest (n=11, Fig. 4J,K), suggesting that AER induction was impaired in the lef1 and tcf7 loss-of-function embryos. At 38 hpf (48 hpf for fgf8), fgf10 was expressed normally in both lef1-MO-injected wild-type and tcf7 mutant embryos (Fig. 4L,M), while expression of the AER markers dlx2a, fgf24, wnt3l and fgf8 was absent from the ectoderm in the MO-injected tcf7 mutants (n=6 each, Fig. 4L-U). The results obtained when wild-type or heterozygous embryos were used for MO injection were essentially indistinguishable (data not shown). From these results, we concluded that Lef7 and Tcf1 are functionally redundant during pectoral fin out growth and play essential role(s) both in the AER induction and maintenance stages.

Characterization of transcripts in the HG21C enhancer trap line
In HG21C, T2KHG was integrated in the coding region in the first exon of the tcf7 gene (Fig. 5A). To understand how the tcf7 gene was disrupted, we performed 3' RACE using nested primers in the first exon. In the HG21C allele, the 3' RACE products were stopped within the insertion (Fig. 5B). The longest transcript had a capacity to produce a truncated protein of 44 amino acids containing the N-terminal region of Tcf7, which is unlikely to be functional. Then, we performed RT-PCR using the f3 and r3 primers to detect possible transcripts that passed over the insertion. Two faint bands that were detected in HG21C homozygous embryos were cloned and sequenced. These bands represented abnormally spliced transcripts containing premature stop codons (Fig. 5C). As a transcript containing a wild-type sequence of the first exon could not be detected, the HG21C allele is likely to be null.

Furthermore, we analyzed how the hsp70 promoter is activated in the enhancer trap lines by 5' RACE. Although the zebrafish hsp70 promoter has been a useful tool (Halloran et al., 2000; Uemura et al., 2005), the transcription start site has not yet been characterized. First, we prepared RNA from heat-shocked HG21C homozygous embryos, and obtained four 5' RACE clones. Three of them contained the same A at the 5' ends, which we designated as position +1, and the other contained A at -2 at the 5' end (Fig. 5D). Second, we prepared RNA from HG21C homozygous embryos at normal temperatures, and sequenced two 5' RACE clones. These contained A at +1 and +2 at their 5' ends (Fig. 5D). Thus, the transcription start sites were nearly the same in both heat-shocked and non heat-shocked conditions, indicating that the hsp70 promoter on T2KHG was indeed activated by a putative tcf7 enhancer in the trap line. The 5' RACE analysis did not amplify the longest 3' RACE product probably because the smaller amount of transcripts that started from the tcf7 promoter. We also analyzed four 5' RACE clones amplified from the HG2A and HG21B lines at normal temperatures. Similar to the 5' RACE products from HG21C, three and one clones contained A at +1 and A at +2 as the 5' ends, respectively. In the course of these analyses, we found an intron in the hsp70 promoter fragment (Fig. 5D). We investigated EST sequences in the database, and found that the endogenous hsp70 gene also contains an intron in the 5' UTR.

View larger version (70K): [in this window] [in a new window]   Fig. 3. The HG21C insertion disrupted the tcf7 gene. (A) The structure of the T2KHG insertion in the tcf7 gene. T2KHG is composed of Tol2 sequences (black), the zebrafish hsp70 promoter (orange), the GFP gene (green) and the SV40 polyA signal (purple). Exons (blue boxes) and 5' UTR (white box) of the tcf7 gene are shown. Black arrows indicate positions and directions of primers. (B) Whole-mount in situ hybridization of an HG21C heterozygous embryo at 24 hpf using the gfp probe. (C) Whole-mount in situ hybridization of a wild-type embryo at 24 hpf using the tcf7 probe. (D-G) The median fin fold of HG21C embryos. Heterozygous (D,F) and homozygous (E,G) embryos at 60 hpf (D,E) and 72 hpf (F,G). (H) Summary of the linkage between the fin phenotype and the GFP expression. (I) Examples of the genotype analysis by PCR using tcf7-f2 and tcf7-r2 (top) and control PCR using tcf7-r2 and Tol2-OUT (bottom). M, DNA size marker; N, no DNA; P, positive control. (J) Summary of the genotype analysis. (K-R) Whole-mount in situ hybridization using the tcf7 probe. Wild-type embryos at 24 hpf (K) and 36 hpf (M), and HG21C homozygous embryos at 24 hpf (L) and 36 hpf (N). The pectoral fin buds of wild-type embryos at 36 hpf (O) and 48 hpf (Q), and HG21C homozygous embryos at 36 hpf (P) and 48 hpf (R). (S,T) The pectoral fins of 72 hpf heterozygous (S) and homozygous (T) HG21C embryos. (U,V) Microinjection of tcf7-MO. The pectoral fin (U) and the median fin (V) of MO-injected HG21 heterozygous embryos at 72 hpf. (W) Summary of the numbers of MO-injected embryos that showed abnormal median fin folds and pectoral fins.

View larger version (47K): [in this window] [in a new window]   Fig. 4. Roles of Tcf7 and Lef1 in the pectoral fin outgrowth. (A-C) Microinjection of lef1-MO into HG21C embryos. The pectoral fins of MO-injected heterozygous (A) and homozygous (B) embryos at 72 hpf. (C) Summary of the numbers of MO-injected embryos that showed an outgrown fin or reduced fin phenotype. (D-U) The pectoral fins of lef1-MO-injected wild-type and HG21C embryos analyzed by whole-mount in situ hybridization. The stages (28 hpf, 36 hpf, 38 hpf and 48 hpf) are shown on the top right. Wild-type (D-H,J,L,N,P,R), heterozygous (T) and homozygous (I,K,M,O,Q,S,U) embryos were used. The probes used are indicated (top right).

View larger version (11K): [in this window] [in a new window]   Fig. 5. Transcripts in the HG21C insertion locus. (A) The structure of the tcf7 locus in wild type and the HG21C enhancer trap line. Blue boxes and a white box indicate exons and 5' UTR, respectively. Positions and directions of primers are shown. (B) Three 3' RACE products (thick lines) identified in homozygous embryos by using nested primers in the first exon. Broken lines indicate regions removed by splicing. (C) Two RT-PCR products (thick lines) identified in homozygous embryos using f3 and r3 primers. Broken lines indicate regions removed by splicing. Positions of premature stop codons are shown (TAA and TGA). (D) The 5' RACE products identified in homozygous embryos in heat-shocked and non heat-shocked conditions by using nested primers in the GFP gene. A broken line indicates an intron. Arrows indicate 5' ends of the 5' RACE products.

In HGn8H, GFP and gfp mRNA was expressed in the anterior ventral diencephalon, midbrain and spinal cord at 24 hpf (Fig. 6J,K). By contrast, the synbl mRNA was accumulated weakly throughout the body (Fig. 6L). To explain this discrepancy, we hypothesized that a putative enhancer that regulates a neighboring gene activated the hsp70 promoter. To test this hypothesis, we cloned cDNA of the rfx4 gene that was located 5 kb upstream of synbl (Fig. 6A). rfx4 encodes a winged helix transcription factor RFX4 which is essential for brain morphogenesis in mice (Blackshear et al., 2003). We found that the rfx4 mRNA was accumulated in the anterior ventral diencephalons and the spinal cord (Fig. 6M), where the strong gfp expression was detected. This result suggested that an rfx4 enhancer activated the hsp70 promoter.

View larger version (76K): [in this window] [in a new window]   Fig. 6. The HGn8H insertion disrupted the synembryn-like gene. (A) The structure of the T2KHG insertion in the synbl locus in the HG8H enhancer trap line. Arrowheads indicate positions and directions of primers. Blue and purple boxes indicate exons of the synbl and rfx4 genes, respectively. White boxes indicate 5' and 3' UTRs. (B-E) The pigment and edema phenotype in HGn8H embryos at day 5. Dorsal and side views of heterozygous (B,C) and homozygous (D,E) embryos. (F) Summary of the link between embryonic lethality and GFP expression. (G) Examples of the genotype analysis by PCR using synbl-f and synbl-r (top) and control PCR using r2 and Tol2-OUT (bottom). M, DNA size marker; N, no DNA; P, positive control. (H) Summary of the genotype analysis. (I) RT-PCR analysis of wild-type, heterozygous and homozygous embryos using synbl-f and r2 (left). Control RT-PCR using ef1-f and ef1-r primers (right). (J,K) GFP expression pattern in 24 hpf heterozygous embryos. GFP fluorescence (J) and whole-mount in situ hybridization using the gfp probe (K). (L,M) Whole-mount in situ hybridization of 24 hpf wild-type embryos using the synbl (L) and rfx4 (M) probes. (N) A phylogenic analysis of vertebrate synembryn homologs. (O,P) Whole-mount in situ hybridization of 24 hpf wild-type embryos using the synbl (O) and ric8a (P) probes. (Q-V) Rescue of the pigment phenotype by forskolin. Pigmentation of heterozygous (Q,T), homozygous (R,U) and synbl-MO-injected wild-type (S,V) embryos at day 5. Embryos were soaked in 1 µM (T,U) and 2 µM (V) forskolin.

Genetic studies have shown that the C. elegans synembryn gene is involved in activation of the G_q and G_S pathway, which lead to production of diacylglycerol and cyclic AMP (cAMP), respectively (Miller et al., 2000; Schade et al., 2005). Biochemical studies have shown that rat RIC8A is a GTP exchange factor for G proteins (Tall et al., 2003). Therefore, the synbl gene may also activate G proteins in zebrafish. Recently, it was reported that dispersion of melanosomes is positively regulated by increase in the cellular cAMP level (Logan et al., 2006). These prompted us to hypothesize that the observed small pigment spot is caused by a decrease in the cAMP level. To test this hypothesis, we treated embryos from HGn8H heterozygous parents with forskolin, an activator of the adenylyl cyclase (Seamon et al., 1981). As application of forskolin to zebrafish embryos suppresses the hedgehog pathway and causes gross morphological defects (Barresi et al., 2000), we optimized its concentration. We found 89% (49/55) of homozygous embryos soaked in 1 µM forskolin formed normally dispersed melanosomes (Fig. 6Q,R,T,U), indicating that the pigment phenotype can be rescued by activating adenylyl cyclase. However, the edema and embryonic lethality were not rescued by the forskolin treatment. We then treated synbl-MO injected embryos with 2 µM forskolin. Eighty-six percent (118/137) of the treated embryos showed normally dispersed melanosomes (Fig. 6S,V), whereas 88% (57/65) of untreated embryos showed small pigment spots. These results suggested that the small pigment spot in the synbl mutant was caused by a decrease in the adenylyl cyclase activity.

	DISCUSSION

TOP SUMMARY INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

 
The efficiency of enhancer trapping using T2KHG
In this study, we identified 125 unique GFP expression patterns from 77 injected fish. This frequency (1.6=125/77) is higher than those reported for other enhancer trap methods; i.e. a Sleeping Beauty construct using the modified EF1 promoter (0.03), a Tol2 construct using the keratin8 promoter (0.12), a retroviral construct using the gata2 promoter (0.3) (Balciunas et al., 2004; Ellingsen et al., 2005; Parinov et al., 2004). We think this is due to the highly efficient germline transmission by the Tol2 transposon system described here (70%), and to the high responsiveness of the hsp70 promoter to chromosomal enhancers. The responsiveness of a minimal promoter to enhancers can be discussed by comparing frequencies to obtain unique GFP expression patterns per insertions. In this study, 125 GFP expression patterns were identified in 256 F1 fish that harbored a total of 215 insertions. Thus, 58% (125/215) of T2KHG insertions caused unique GFP expression patterns. By contrast, in the enhancer trap screens using the keratin8, modified EF1 and gata2 promoter, this frequency was estimated as 28%, 4% and 14%, respectively (Amsterdam and Becker, 2005; Kawakami, 2005). In Drosophila, the hsp70, P-transposase and ftz promoters have been used as minimal promoters for enhancer trap constructs. It was shown that 90%, 20% and 40% of insertions of these constructs caused lacZ expression, respectively (Mlodzik and Hiromi, 1992). Thus, both in zebrafish and Drosophila, the hsp70 promoter exhibited the highest enhancer trap activity. A possible disadvantage caused by using the hsp70 promoter may be its basal transcription activity. We are currently dissecting the zebrafish hsp70 promoter to remove elements regulating those unwanted basal activities.

Although the hsp70 promoter was used for an enhancer trap screen reported recently (Scott et al., 2007), its mechanism of action has not been characterized. We demonstrated that the hsp70 promoter is indeed activated in the enhancer trap lines, strengthening its usefulness as a minimal promoter. In the Drosophila and human hsp70 promoters, short RNA transcripts are produced at the transcription start site in uninduced conditions, and elongation of the paused transcript is stimulated upon heat shock (Brown et al., 1996; Rougvie and Lis, 1988). The zebrafish hsp70 promoter has not yet been characterized in such a detail. However, the observed common feature, the high responsiveness to enhancers, may suggest that a similar mechanism also operates the zebrafish hsp70 promoter. It is interesting that, unlike Drosophila and human, the zebrafish hsp70 promoter is TATA-less as there is no TATA sequence upstream of the identified transcription start site. Based on the information about the transcription start site as well as the intron in the 5' UTR, we aim to construct improved versions of enhancer trap constructs with minimum basal activities.

We found that, in the case of HGn8H, the hsp70 promoter on T2KHG integrated in the synbl gene was probably activated by an enhancer of its neighboring gene: rfx4. A similar phenomenon has been described also in retroviral enhancer trapping (Kikuta et al., 2007). How was the hsp70 promoter affected by an rfx4 enhancer but not by a synbl enhancer? How did the rfx4 enhancer affect the hsp70 promoter while not affecting the synbl promoter in a wild-type condition? Studies on the rfx4 and synbl enhancers and promoters may illuminate an unknown mechanism that governs specificity between enhancer and promoter.

Roles of Tcf7 and Lef1 in AER formation
We found that Tcf7 and Lef1 are essential for expression of AER markers in the ectoderm in the early and late stages of the pectoral fin development. It has been shown that, in the early limb/fin induction stage, Wnt2b, which is expressed in the lateral plate mesoderm (LPM), activates expression of fgf10 in the mesenchyme of the limb/fin buds in chicken and zebrafish (Kawakami et al., 2001; Ng et al., 2002). In mouse, although Wnt2b expression was not detected in LPM, Fgf10 expression became weaker in Lef1^-/-;Tcf7^-/- embryos and it was suggested that signaling mediated by unidentified Wnt(s) is required to maintain normal levels of Fgf10 expression (Agarwal et al., 2003). By contrast, our present study indicated that Lef1 and Tcf7 are not required for the mesenchymal fgf10 expression in zebrafish. Thus, components of Wnt signaling involved in Fgf10 induction are species specific and additional Tcf genes may compensate the loss of tcf7 and lef1 in zebrafish. In addition, our loss-of-function study suggested that the Wnt signaling in the ectoderm mediated by Lef1 and Tcf7 is essential for AER maintenance. This notion is consistent with the previous observations that Wnt3a-mediated β-catenin-dependent signaling activates expression of AER markers in the chicken limb ectoderm (Kawakami et al., 2001; Kengaku et al., 1998) and mouse Lef1^-/-;Tcf7^-/- embryos exhibit a defect in limb development (Galceran et al., 1999).

As tcf7 is exclusively expressed also in the dorsal retina, it can be speculated that Tcf7 may have a unique role also in this area (Fig. 3B,C) (Veien et al., 2005). At present, however, we have not detected any obvious defects in the dorsal retina (M. Yamaguchi, I. Masai, E. S. Veien and R. Dorsky, personal communications). It has been shown that the same factors, such as Dlx genes, fgf24 and sp9, are expressed both in the AER and the edge of the median fin fold (Abe et al., 2007). Although a mechanism that regulates outgrowth of the median fin folds is largely unknown, we noticed that outgrowth of the median fins was also impaired in the lef1 and tcf7 loss-of-function embryos (data not shown), suggesting that similar Wnt and Fgf signaling pathways regulate development of both pectoral fins and median fin folds.

The zebrafish synembryn-like gene activates the G_S pathway
It has been shown that synembryn and its mammalian homologs are involved in activation of G proteins (Klattenhoff et al., 2003; Miller et al., 2000; Schade et al., 2005; Tall et al., 2003). Recently, in zebrafish, it was shown that dispersion of melanosomes is enhanced by activation of adenylyl cyclase (Logan et al., 2006). Our study established a link between these two processes. The disruption of the synbl function caused aggregation of melanosomes, which could be restored by activation of adenylyl cyclase. Therefore, it is reasonable to postulate that the synbl gene, a homolog of mammalian RIC8B, is involved in activation of the G_S pathway, leading to activation of adenylyl cyclase and dispersion of melanosomes. The synbl gene may be involved in regulation of pigmentation in wild-type conditions, such as a physiological color change during background adaptation. However, the edema phenotype and the embryonic lethality were not rescued by the forskolin treatment. The concentration of forskolin may not be high enough to rescue those phenotypes, or alternatively, those phenotypes may be caused by failures in activation of other G proteins, such as G_q, which is known to bind to human RIC8B in vitro (Klattenhoff et al., 2003).

Insertional mutagenesis by enhancer trapping
In this study, we isolated two phenotypic mutants out of 54 enhancer trap insertions. Although this frequency is not far superior to that with retroviral insertional mutagenesis in which one in 80 insertions caused embryonic lethality (Amsterdam et al., 1999), we think insertional mutagenesis by enhancer trapping should have the following merits. First, only a small number of F1 fish that show interesting GFP expression patterns need to be raised. Second, as heterozygous fish carrying same insertions can be identified in the F1 generation, it is not necessary to raise a large number of F2 fish, and, instead, homozygous phenotypes can be detected by analyzing F2 embryos. Third, as the place to be analyzed is illuminated by GFP, subtle morphological defects, such as fin phenotypes in the tcf7 mutant, can be identified. Finally, as insertions are `visible', carriers can be easily maintained without time-consuming genotyping. We demonstrated that our enhancer trap construct can be integrated within transcribed regions at a relatively high frequency. It is higher than that calculated for retroviral enhancer trap insertions, although it is not statistically different from that calculated for random integration. This finding opened a possibility that insertional mutagenesis could be performed more efficiently if an enhancer trap construct that can disrupt the function of target genes more efficiently was developed; for example, development of enhancer trap constructs carrying more elements to interfere with endogenous transcripts, such as a splice acceptor plus a polyA signal, etc. Studies along this line are in progress in our laboratory. In conclusion, our present study provided a basis for the development of efficient transposon-mediated insertional mutagenesis in a vertebrate.

Supplementary material
Supplementary material for this article is available at http://dev.biologists.org/cgi/content/full/135/1/159/DC1

	ACKNOWLEDGMENTS

 
We thank R. Dorsky for helpful discussion, and T. Uematsu, N. Mouri, S. Takeda, R. Mimura and M. Mizushina for fish room works. This work was supported by NIH R01 GM69382 and National BioResource Project, and by grants from the Ministry of Education, Culture, Sports, Science and Technology of Japan.

	Footnotes

 
^* Present address: Research Institute for Electronic Science, Hokkaido University, Sapporo 060-0812, Japan

	REFERENCES

TOP SUMMARY INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

 

Abe, G., Ide, H. and Tamura, K. (2007). Function of FGF signaling in the developmental process of the median fin fold in zebrafish. Dev. Biol. 304,355 -366.[CrossRef][Medline]

Agarwal, P., Wylie, J. N., Galceran, J., Arkhitko, O., Li, C., Deng, C., Grosschedl, R. and Bruneau, B. G. (2003). Tbx5 is essential for forelimb bud initiation following patterning of the limb field in the mouse embryo. Development 130,623 -633.[Abstract/Free Full Text]

Akimenko, M. A., Ekker, M., Wegner, J., Lin, W. and Westerfield, M. (1994). Combinatorial expression of three zebrafish genes related to distal-less: part of a homeobox gene code for the head. J. Neurosci. 14,3475 -3486.[Abstract]

Amsterdam, A. and Becker, T. S. (2005). Transgenes as screening tools to probe and manipulate the zebrafish genome. Dev. Dyn. 234,255 -268.[CrossRef][Medline]

Amsterdam, A., Burgess, S., Golling, G., Chen, W., Sun, Z., Townsend, K., Farrington, S., Haldi, M. and Hopkins, N. (1999). A large-scale insertional mutagenesis screen in zebrafish. Genes Dev. 13,2713 -2724.[Abstract/Free Full Text]

Amsterdam, A., Nissen, R. M., Sun, Z., Swindell, E. C., Farrington, S. and Hopkins, N. (2004). Identification of 315 genes essential for early zebrafish development. Proc. Natl. Acad. Sci. USA 101,12792 -12797.[Abstract/Free Full Text]

Balciunas, D., Davidson, A. E., Sivasubbu, S., Hermanson, S. B., Welle, Z. and Ekker, S. C. (2004). Enhancer trapping in zebrafish using the Sleeping Beauty transposon. BMC Genomics 5,62 .[CrossRef][Medline]

Barresi, M. J., Stickney, H. L. and Devoto, S. H. (2000). The zebrafish slow-muscle-omitted gene product is required for Hedgehog signal transduction and the development of slow muscle identity. Development 127,2189 -2199.[Abstract]

Blackshear, P. J., Graves, J. P., Stumpo, D. J., Cobos, I., Rubenstein, J. L. and Zeldin, D. C. (2003). Graded phenotypic response to partial and complete deficiency of a brain-specific transcript variant of the winged helix transcription factor RFX4. Development 130,4539 -4552.[Abstract/Free Full Text]

Brown, S. A., Imbalzano, A. N. and Kingston, R. E. (1996). Activator-dependent regulation of transcriptional pausing on nucleosomal templates. Genes Dev. 10,1479 -1490.[Abstract/Free Full Text]

Driever, W., Solnica-Krezel, L., Schier, A. F., Neuhauss, S. C., Malicki, J., Stemple, D. L., Stainier, D. Y., Zwartkruis, F., Abdelilah, S., Rangini, Z. et al. (1996). A genetic screen for mutations affecting embryogenesis in zebrafish. Development 123, 37-46.[Abstract]

Ellingsen, S., Laplante, M. A., Konig, M., Kikuta, H., Furmanek, T., Hoivik, E. A. and Becker, T. S. (2005). Large-scale enhancer detection in the zebrafish genome. Development 132,3799 -3811.[Abstract/Free Full Text]

Felsenstein, J. (1985). Confidence limits on phylogenies: an approach using the bootstrap. Evolution 39,783 -791.[CrossRef]

Fischer, S., Draper, B. W. and Neumann, C. J. (2003). The zebrafish fgf24 mutant identifies an additional level of Fgf signaling involved in vertebrate forelimb initiation. Development 130,3515 -3524.[Abstract/Free Full Text]

Gaiano, N., Amsterdam, A., Kawakami, K., Allende, M., Becker, T. and Hopkins, N. (1996). Insertional mutagenesis and rapid cloning of essential genes in zebrafish. Nature 383,829 -832.[CrossRef][Medline]

Galceran, J., Farinas, I., Depew, M. J., Clevers, H. and Grosschedl, R. (1999). Wnt3a-/--like phenotype and limb deficiency in Lef1(-/-)Tcf1(-/-) mice. Genes Dev. 13,709 -717.[Abstract/Free Full Text]

Haffter, P., Granato, M., Brand, M., Mullins, M. C., Hammerschmidt, M., Kane, D. A., Odenthal, J., van Eeden, F. J., Jiang, Y. J., Heisenberg, C. P. et al. (1996). The identification of genes with unique and essential functions in the development of the zebrafish, Danio rerio. Development 123,1 -36.[Abstract]

Halloran, M. C., Sato-Maeda, M., Warren, J. T., Su, F., Lele, Z., Krone, P. H., Kuwada, J. Y. and Shoji, W. (2000). Laser-induced gene expression in specific cells of transgenic zebrafish. Development 127,1953 -1960.[Abstract]

Kawakami, K. (2004). Transgenesis and gene trap methods in zebrafish by using the Tol2 transposable element. Methods Cell Biol. 77,201 -222.[Medline]

Kawakami, K. (2005). Transposon tools and methods in zebrafish. Dev. Dyn. 234,244 -254.[CrossRef][Medline]

Kawakami, K. and Shima, A. (1999). Identification of the Tol2 transposase of the medaka fish Oryzias latipes that catalyzes excision of a nonautonomous Tol2 element in zebrafish Danio rerio. Gene 240,239 -244.[CrossRef][Medline]

Kawakami, K., Koga, A., Hori, H. and Shima, A. (1998). Excision of the Tol2 transposable element of the medaka fish, Oryzias latipes, in zebrafish, Danio rerio. Gene 225, 17-22.[CrossRef][Medline]

Kawakami, K., Shima, A. and Kawakami, N. (2000). Identification of a functional transposase of the Tol2 element, an Ac-like element from the Japanese medaka fish, and its transposition in the zebrafish germ lineage. Proc. Natl. Acad. Sci. USA 97,11403 -11408.[Abstract/Free Full Text]

Kawakami, Y., Capdevila, J., Buscher, D., Itoh, T., Rodriguez Esteban, C. and Izpisua Belmonte, J. C. (2001). WNT signals control FGF-dependent limb initiation and AER induction in the chick embryo. Cell 104,891 -900.[CrossRef][Medline]

Kawakami, K., Takeda, H., Kawakami, N., Kobayashi, M., Matsuda, N. and Mishina, M. (2004). A transposon-mediated gene trap approach identifies developmentally regulated genes in zebrafish. Dev. Cell 7,133 -144.[CrossRef][Medline]

Kengaku, M., Capdevila, J., Rodriguez-Esteban, C., De La Pena, J., Johnson, R. L., Belmonte, J. C. and Tabin, C. J. (1998). Distinct WNT pathways regulating AER formation and dorsoventral polarity in the chick limb bud. Science 280,1274 -1277.[Abstract/Free Full Text]

Kent, W. J. (2002). BLAT-the BLAST-like alignment tool. Genome Res. 12,656 -664.[Abstract/Free Full Text]

Kikuta, H., Laplante, M., Navratilova, P., Komisarczuk, A. Z., Engstrom, P. G., Fredman, D., Akalin, A., Caccamo, M., Sealy, I., Howe, K. et al. (2007). Genomic regulatory blocks encompass multiple neighboring genes and maintain conserved synteny in vertebrates. Genome Res. 17,545 -555.[Abstract/Free Full Text]

Klattenhoff, C., Montecino, M., Soto, X., Guzman, L., Romo, X., Garcia, M. A., Mellstrom, B., Naranjo, J. R., Hinrichs, M. V. and Olate, J. (2003). Human brain synembryn interacts with Gsalpha and Gqalpha and is translocated to the plasma membrane in response to isoproterenol and carbachol. J. Cell. Physiol. 195,151 -157.[CrossRef][Medline]

Kotani, T., Nagayoshi, S., Urasaki, A. and Kawakami, K. (2006). Transposon-mediated gene trapping in zebrafish. Methods 39,199 -206.[CrossRef][Medline]

Logan, D. W., Burn, S. F. and Jackson, I. J. (2006). Regulation of pigmentation in zebrafish melanophores. Pigment Cell Res. 19,206 -213.[CrossRef][Medline]

Miller, K. G., Emerson, M. D., McManus, J. R. and Rand, J. B. (2000). RIC-8 (Synembryn): a novel conserved protein that is required for G (q)alpha signaling in the C. elegans nervous system. Neuron 27,289 -299.[CrossRef][Medline]

Mlodzik, M. and Hiromi, Y. (1992). Enhancer trap method in Drosophila: its application to neurobiology. In Methods in Neurosciences. Vol.9 (ed. P. M. Conn), pp.397 -414. San Diego: Academic Press.

Ng, J. K., Kawakami, Y., Buscher, D., Raya, A., Itoh, T., Koth, C. M., Rodriguez Esteban, C., Rodriguez-Leon, J., Garrity, D. M., Fishman, M. C. et al. (2002). The limb identity gene Tbx5 promotes limb initiation by interacting with Wnt2b and Fgf10. Development 129,5161 -5170.[Medline]

Norton, W. H., Ledin, J., Grandel, H. and Neumann, C. J. (2005). HSPG synthesis by zebrafish Ext2 and Extl3 is required for Fgf10 signalling during limb development. Development 132,4963 -4973.[Abstract/Free Full Text]

Parinov, S., Kondrichin, I., Korzh, V. and Emelyanov, A. (2004). Tol2 transposon-mediated enhancer trap to identify developmentally regulated zebrafish genes in vivo. Dev. Dyn. 231,449 -459.[CrossRef][Medline]

Reifers, F., Bohli, H., Walsh, E. C., Crossley, P. H., Stainier, D. Y. and Brand, M. (1998). Fgf8 is mutated in zebrafish acerebellar (ace) mutants and is required for maintenance of midbrain-hindbrain boundary development and somitogenesis. Development 125,2381 -2395.[Abstract]

Rougvie, A. E. and Lis, J. T. (1988). The RNA polymerase II molecule at the 5' end of the uninduced hsp70 gene of D. melanogaster is transcriptionally engaged. Cell 54,795 -804.[CrossRef][Medline]

Rzhetsky, A. and Nei, M. (1992). Statistical properties of the ordinary least-squares, generalized least-squares, and minimum-evolution methods of phylogenetic inference. J. Mol. Evol. 35,367 -375.[CrossRef][Medline]

Saitou, N. and Nei, M. (1987). The neighbor-joining method: a new method for reconstructing phylogenetic trees. Mol. Biol. Evol. 4,406 -425.[Abstract]

Schade, M. A., Reynolds, N. K., Dollins, C. M. and Miller, K. G. (2005). Mutations that rescue the paralysis of Caenorhabditis elegans ric-8 (synembryn) mutants activate the G alpha (s) pathway and define a third major branch of the synaptic signaling network. Genetics 169,631 -649.[Abstract/Free Full Text]

Scott, E. K., Mason, L., Arrenberg, A. B., Ziv, L., Gosse, N. J., Xiao, T., Chi, N. C., Asakawa, K., Kawakami, K. and Baier, H. (2007). Targeting neural circuitry in zebrafish using GAL4 enhancer trapping. Nat. Methods 4, 323-326.[Medline]

Seamon, K. B., Padgett, W. and Daly, J. W. (1981). Forskolin: unique diterpene activator of adenylate cyclase in membranes and in intact cells. Proc. Natl. Acad. Sci. USA 78,3363 -3367.[Abstract/Free Full Text]

Tall, G. G., Krumins, A. M. and Gilman, A. G. (2003). Mammalian Ric-8A (synembryn) is a heterotrimeric Galpha protein guanine nucleotide exchange factor. J. Biol. Chem. 278,8356 -8362.[Abstract/Free Full Text]

Thompson, J. D., Higgins, D. G. and Gibson, T. J. (1994). CLUSTAL W: improving the sensitivity of progressive multiple sequence alignment through sequence weighting, position-specific gap penalties and weight matrix choice. Nucleic Acids Res. 22,4673 -4680.[Abstract/Free Full Text]

Uemura, O., Okada, Y., Ando, H., Guedj, M., Higashijima, S., Shimazaki, T., Chino, N., Okano, H. and Okamoto, H. (2005). Comparative functional genomics revealed conservation and diversification of three enhancers of the isl1 gene for motor and sensory neuron-specific expression. Dev. Biol. 278,587 -606.[CrossRef][Medline]

Urasaki, A., Morvan, G. and Kawakami, K. (2006). Functional dissection of the Tol2 transposable element identified the minimal cis-sequence and a highly repetitive sequence in the subterminal region essential for transposition. Genetics 174,639 -649.[Abstract/Free Full Text]

Veien, E. S., Grierson, M. J., Saund, R. S. and Dorsky, R. I. (2005). Expression pattern of zebrafish tcf7 suggests unexplored domains of Wnt/beta-catenin activity. Dev. Dyn. 233,233 -239.[CrossRef][Medline]

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