The Berkeley Drosophila Genome Project Gene Disruption Project: Single P-Element Insertions Mutating 25% of Vital Drosophila Genes

Corresponding author: Allan C. Spradling, Howard Hughes Medical Institute Research Laboratories, Department of Embryology, Carnegie Institution of Washington, 115 W. University Pkwy., Baltimore, MD 21210., spradling{at}mail1.ciwemb.edu (E-mail)

Communicating editor: R. S. HAWLEY

	ABSTRACT

TOP ABSTRACT MATERIALS AND METHODS RESULTS DISCUSSION LITERATURE CITED

A fundamental goal of genetics and functional genomics is to identify and mutate every gene in model organisms such as Drosophila melanogaster. The Berkeley Drosophila Genome Project (BDGP) gene disruption project generates single P-element insertion strains that each mutate unique genomic open reading frames. Such strains strongly facilitate further genetic and molecular studies of the disrupted loci, but it has remained unclear if P elements can be used to mutate all Drosophila genes. We now report that the primary collection has grown to contain 1045 strains that disrupt more than 25% of the estimated 3600 Drosophila genes that are essential for adult viability. Of these P insertions, 67% have been verified by genetic tests to cause the associated recessive mutant phenotypes, and the validity of most of the remaining lines is predicted on statistical grounds. Sequences flanking >920 insertions have been determined to exactly position them in the genome and to identify 376 potentially affected transcripts from collections of EST sequences. Strains in the BDGP collection are available from the Bloomington Stock Center and have already assisted the research community in characterizing >250 Drosophila genes. The likely identity of 131 additional genes in the collection is reported here. Our results show that Drosophila genes have a wide range of sensitivity to inactivation by P elements, and provide a rationale for greatly expanding the BDGP primary collection based entirely on insertion site sequencing. We predict that this approach can bring >85% of all Drosophila open reading frames under experimental control.

THE nucleotide sequences of several complex eukaryotic genomes, including those of Caenorhabditis elegans, Drosophila melanogaster, Arabidopsis thaliana, Mus musculus, and Homo sapiens, are virtually complete or scheduled for completion during the next several years (COLLINS et al. 1998 ; MEINKE et al. 1998 ). Large-scale sequencing of human and model organism genomes, cDNAs, and expressed sequence tags (ESTs) is identifying tens of thousands of genes about which little is known. Obtaining mutations in these loci on chromosomes free of additional lesions is essential for their functions to be deduced using model organisms. However, mutations in particular open reading frames must still usually be obtained in piecemeal fashion, by producing specifically tailored gene knockouts or by identifying the desired strains within large, randomly mutagenized collections. Both approaches remain slow and uncertain. These problems could be circumvented by constructing complete mutation libraries, whose strains each disrupt single distinct genes. Genome-wide collections of gene knockouts would provide a vital resource for gene-based approaches to biological research.

Insertional mutagenesis provides a highly advantageous strategy for constructing mutations in advance throughout entire genomes, because it simplifies the problem of determining which genes have been disrupted. Insertional screens at low multiplicity have been carried out in bacteria (KLECKNER et al. 1977 ), yeast (BURNS et al. 1994 ; GARRAWAY et al. 1997 ), Arabidopsis (SUNDARESAN et al. 1995 ; BHATT et al. 1996 ; SMITH et al. 1996 ), C. elegans (PLASTERK 1993 ; KORSWAGEN et al. 1996 ), Drosophila (COOLEY et al. 1988 ; RORTH 1996 ), zebrafish (ALLENDE et al. 1996 ; GAIANO et al. 1996 ), and mice (JAENISCH 1988 ; GOSSLER et al. 1989 ; WURST et al. 1995 ; ZAMBROWICZ et al. 1998 ). However, converting the products of raw screens into a complete mutation library is a challenging task. The site selectivity of the mutagenic element must be extremely broad to target all genes. High throughput methods must be developed and used to identify screen products that contain single insertions located within distinct genes, because strains bearing just one new insertion each are needed to assess gene function. Consequently, it remains uncertain whether it is possible in practice to construct a complete library of mutations using this approach.

Among model multicellular eukaryotes, insertional mutagenesis has been used for genetic analysis and functional genomics most extensively in Drosophila. Low-multiplicity mutageneses using engineered P elements have been carried out frequently (COOLEY et al. 1988 ; BELLEN et al. 1989 ; BIER et al. 1989 ; BERG and SPRADLING 1991 ; KARPEN and SPRADLING 1992 ; GAUL et al. 1992 ; TOROK et al. 1993 ; CHANG et al. 1993 ; ERDELYI et al. 1995 ; RORTH 1996 ; DEAK et al. 1997 ; SOZEN et al. 1997 ; RORTH et al. 1998 ). While the raw strain collections produced in such studies are highly redundant and contain lines with multiple mutations, they provide ideal starting material for constructing a genome-wide mutation library. In 1993, the Berkeley Drosophila Genome Project (BDGP) gathered ~3900 lines associated with mutant phenotypes (mostly lethality) from seven existing raw collections and began to construct a gene disruption library for use by the Drosophila research community (SPRADLING et al. 1995 ). The Drosophila genome is thought to contain ~3600 vital genes (MIKLOS and RUBIN 1996 ), so the project had the potential to encompass a substantial fraction of genes that can mutate to a phenotype recognizable in large laboratory screens (primarily lethality). In contrast, the total number of genes is thought to be about three times larger (MIKLOS and RUBIN 1996 ). The analysis of these collections also promised to indicate the feasibility of eventually using P-element insertional mutagenesis to disrupt all Drosophila genes.

The seven initial collections have now been analyzed, and we document here a library of strains that disrupts ~1000 different genes. A total of 450 of the strains mutate genes that have been described previously in Drosophila or represent novel loci defined by homology to well-studied genes in other organisms. These associations were made with the assistance of researchers throughout the Drosophila community who have used the collection to help characterize >250 genes, and through the efforts of the BDGP project, including 138 new gene-mutation links reported here. Another 135 disrupted genes are associated only with EST sequences that predict novel proteins or products related to proteins of unknown function in other organisms. An additional 138 lines are inserted within sequenced regions containing candidate open reading frames (ORFs). Thus, >700 of the 1045 mutant strains already link mutant phenotypes with specific open reading frames, and the remaining lines only await completion of the genomic DNA sequence. The ~1000 genes already represented in the library constitute ~25% of all Drosophila genes readily defined by mutation, and specify more gene-mutation links than are currently available in other model multicellular eukaryotes. Most important, on the basis of this work we have developed a new program to disrupt the remaining genes while the Drosophila genome sequence is being completed and annotated (see Table 1).

	MATERIALS AND METHODS

TOP ABSTRACT MATERIALS AND METHODS RESULTS DISCUSSION LITERATURE CITED

Drosophila strains:
Flies were grown on standard corn meal/agar media (ASHBURNER 1990 ) at 22°. Approximately 3900 lethal, semilethal, sterile, semisterile, or visible lines (Table 2) were collected from seven P-element screens (COOLEY et al. 1988 ; BIER et al. 1989 ; GAUL et al. 1992 ; KARPEN and SPRADLING 1992 ; CHANG et al. 1993 ; TOROK et al. 1993 ; M. SCOTT and M. FULLER, unpublished results) as described (SPRADLING et al. 1995 ). Three different P-element vectors were used: PZ[ry] (MLODZIK et al. 1990 ), Plac W (BIER et al. 1989 ), or Puc-hsneo (STELLER and PIRROTTA 1986 ). About 40% of the starting lines were marked with rosy⁺ and 60% with white⁺. The GAUL et al. 1992 collection was stained for enhancer trap patterns in third instar larval eye-antenna imaginal discs, and only lines showing expression were analyzed further. Lines from the TOROK et al. 1993 screen that share the first three numbers in their designator (see Nomenclature) were obtained from the same parents and may derive from premeiotic clusters. When two or more such lines were found to contain insertions at the same polytene site, only one was retained and the other(s) was treated as a duplicate(s). Many lines containing multiple insertions from this screen were discarded prior to localization because they exhibited a diagnostic strong eye coloration.

Deficiency strains were obtained from the Bloomington Stock Center and from many individual laboratories. The deficiencies used are listed in Table 3.

Strain names: BDGP strain names start with a prefix that indicates the chromosome and phenotypic effect of their single P-element insertion. For example, third chromosome strain names begin with either "l(3)" (lethal or strong semilethal), "fs(3)" (female sterile or strong semisterile), "ms(3)" (male sterile or strong semisterile), "v(3)" (visible), or "n(3)" (no obvious phenotype). Semilethal and semisterile mutations were utilized only if they were strong enough to score in complementation tests. Only the effect of the P insertion, not of any secondary mutations on the same chromosome, whether present initially or acquired later, is indicated by the prefix. The phenotypic prefix is followed by a unique designator to distinguish individual lines and to preserve the original names of the lines. Designators for lines from COOLEY et al. 1988 take the form "neo" and a 1–3 digit number ("neo63"); from KARPEN and SPRADLING 1992 , lines retain their original names ("06253"); from BIER et al. 1989 , the letter "j" precedes the original name (i.e., "5C2" becomes "j5C2"); from GAUL et al. 1992 , the letter "r" is contained within the original name (i.e., "rJ713"); from TOROK et al. 1993 , the letter "k" precedes the original name and the slash is omitted (i.e., "133/45" becomes "k13345"); from the Scott and Fuller screen, the letter "s" precedes the original name (i.e., "1629" becomes "s1629"); and for regular names from CHANG et al. 1993 , the L is moved to the start, the R omitted, and a zero added after the number (i.e., "534RL" becomes "L5340"). While the phenotypic prefix may rarely be changed to reflect new information about the effect of the P insertion, the designator is invariant. Thus, l(2)06253 and n(2)06253 refer to a single BDGP strain, whose P insertion was initially thought to cause lethality, but was subsequently shown to cause no obvious phenotype. Because phenotypic prefixes can change, it is wise to search Internet databases using the designator. Periodically updated information on the BDGP strains can be obtained by searching the BDGP website at http://www.fruitfly.org/p_disrupt/, or from FlyBase (the Drosophila database project) at http://flybase.bio.indiana.edu/transposons/fbinsquery.hform.

Gene names: Symbols for Drosophila gene names are as given by FlyBase. For potentially novel loci defined only by a BDGP insertion strain, the name of the primary strain constitutes the provisional gene name, in accordance with FlyBase rules. Allele names for all the mutations are represented using the designator as the allele superscript. For example, because strain l(2)k10325 is part of the complementation group whose primary strain is l(2)03350 defining a new gene, its mutation is designated l(2)03350^k10325. The P-element mutation in strain l(2)s4771 that is allelic to kismet (kis) is designated kis^s4771. Again, because it is the designator that is presented in allele tables, it is wise to search FlyBase with the wild-carded designator.

Localization of inserts by in situ hybridization:
P elements were localized by in situ hybridization to polytene chromosomes as described previously (SPRADLING et al. 1995 ); see also http://www.fruitfly.org/methods. Digitized images of these localizations are available at http://www.fruitfly.org/p_disrupt/. A few lines were localized by others; these were assumed to be less accurate and are given only to a polytene lettered section, rather than a range of specific bands. To reduce the number of in situ localizations, many alleles of seven known hotspots were removed from the TOROK et al. 1993 collection by complementing each starting strain with the following tester loci: 1(2)07815 (kis), l(2)01209 (vkg), l(2)04208 (Eif4A), l(2)02657 (wg), l(2)00255 (bun), l(2)00642 (lola), and l(2)03505 (mam). The insertion(s) in lines that failed to complement were not localized, and they are not included in the tabulation of hotspot allele numbers. Consequently, the allele numbers for these loci are lower than would have otherwise been the case.

Complementation testing:
Complementation crosses were carried out among single-insertion lines whose insertions were localized within six to eight polytene bands of each other. A two-stage strategy was used to limit the number of crosses and to minimize redundancy. Each line was first crossed to representative of any locus within range having multiple alleles. Lines failing to complement were identified as additional alleles and eliminated from further crosses. Lines not allelic to such local "hotspots" were subsequently crossed to representatives of the other complementation groups within the relevant zone. As soon as two complementation groups were joined, it was assumed that their behavior was uniform, and few additional crosses between the subgroups were carried out. Generally this strategy worked well. However, in a small number of cases, incomplete or inconsistent complementation behavior was observed due to localization errors larger than four to eight bands, to intergenic complementation, to semilethality, to inadvertent selection of a rearranged allele as the representative allele, to stock instability, or to errors in obtaining or recording complementation data. Problem complementation groups were reanalyzed on a case-by-case basis and the source of the contradiction resolved.

Verification:
Strains from the primary collection were crossed to deficiencies (see Table 3) to verify that the P insertion caused the recessive phenotype. In 1717 single-insert strains, the cytogenetic locus of the P element clearly fell within the boundaries of existing deficiency (Df) chromosomes (Table 2). An uncertainty of four to six bands in the cytogenetic breakpoints was assumed, and the previous results of complementation tests with verified lines in the region were also considered (see SPRADLING et al. 1995 ). Complementation with deficiencies that unequivocally remove the P insertion site was taken as proof that the P element did not cause the associated phenotype. Failure to complement indicated that the strain was "verified." While lines with secondary mutations closely linked to the P insertion might be erroneously verified by this procedure, further molecular and genetic analyses suggest that the frequency of such errors is small. The results of the complementation and verification crosses are summarized in Table 2, Table 4, and Table 5. The data are also available on the BDGP website (http://www.fruitfly.org/p_disrupt/).

The availability of DNA sequence information that can link insertion sites to nearby ESTs, transcripts, and predicted genes is expected to significantly change the way decisions to retain or discard lines are made. Except within the Adh region (ASHBURNER et al. 1999 ), we retained insertions only if they caused or were likely to cause a detectable mutant phenotype. However, in the future, as genomic sequences become more highly annotated, it will increasingly be possible to select strains solely on the basis of whether they are likely to disrupt a novel ORF, regardless of whether a recessive phenotype can be observed. In a few cases reported here, viable insertions reside near or within novel transcripts recognized by nucleotide sequence. The prefixes of these lines were changed to n(2) or n(3) to indicate the absence of a scorable phenotype. Only within the Adh region, where sequence annotation is now extensive (ASHBURNER et al. 1999 ), did a significant fraction of the retained lines lack strong phenotypes.

Flanking sequence determination:
Flanking sequences from one or both ends of most P-element insertions in the primary collection were determined by one or both of two methods. Plasmids containing the 5' P element and flanking genomic sequences were rescued from many strains. Prior to rescue, the line was expanded, and 40–100 adult flies were collected and frozen at -20°. The plasmid rescue procedure (based on HAMILTON et al. 1991 ) entails macerating 30–40 flies in a grinding buffer, then one cycle of freeze-thaw, followed by a 20-min incubation at 70°. Subsequently, residual proteins and SDS were removed by addition of potassium acetate (KOAc) and incubation on ice for 30 min. The supernatant obtained after removal of particulate matter was ethanol precipitated to recover genomic DNA. Finally, the samples were treated with RNase A at 37° for 2 hr.

For plasmid rescue, a sample of genomic DNA equivalent to two to four flies was digested with an appropriate restriction enzyme (e.g., XbaI for the PZ lines), then ligated at low DNA concentration to circularize the restriction fragments. Subsequently, DH10B cells were transformed by electroporation. The resulting colonies had acquired the circularized restriction fragment containing the selectable marker, the bacterial origin of replication, one P-element inverted repeat, and a variable amount of flanking genomic DNA. For each rescue, four to six transformants were screened by DNA miniprep and restriction digestion. In cases where at least three of the four (or five of the six) transformants exhibited identical patterns, a plasmid was chosen for sequencing that represented the major class. Occasionally, the appropriate plasmid was identified from a transformation experiment that yielded more than one plasmid form by in situ hybridization. These plasmids were sequenced directly using a primer designed to the P-element inverted repeat. The success rate in this procedure was ~80%.

The remaining lines were analyzed by recovering a smaller amount of DNA using inverse PCR according to the method of J. Rehm (http://www.fruitfly.org/methods/). This method was successfully adapted to a 96-well format where the success rate in obtaining 25 bp or more of flanking sequences has been >85%.

Association with ESTs:
BDGP is generating a collection of 80,000 Drosophila EST sequences with support from Howard Hughes Medical Institute (accessible at http://www.fruitfly.org/EST/). During the preparation of this article, ~48,000 ESTs were available for comparison. Each flanking sequence was searched against this EST database, matches validated by inspection, and the position of the P insertion relative to the EST-homologous portion of the flanking sequence determined. The names of ESTs with strong matches are given in Table 4 and Table 5. Only ESTs that were located within ~100 bp of the P element are reported; more distant sequence matches might represent adjacent transcripts and were not included in the tables.

Stock distribution:
To hasten the availability of the gene disruptions, verified lines from the primary collection were sent to the Bloomington Stock Center in several batches beginning in 1993; the number of strains reached 700 by late in 1994. All 1052 primary collection strains have been available from the Bloomington Stock Center since October 1997. Reserve alleles are maintained at the Carnegie Institution (chromosome 3) or at Berkeley (chromosome 2), and have also been available on request since 1993. Information about stocks is updated periodically on the BDGP website and strains found to be inappropriate are removed from the Bloomington Stock Center. Information derived from further study of any of the BDGP stocks is welcome and should be forwarded to the corresponding author's e-mail address.

Statistical analysis of saturation:
Previous attempts to estimate the saturation behavior of P elements have utilized inadequately characterized data sets. We focused on the 737 independent lines from chromosome 2 and 535 independent lines from chromosome 3 that contain a single verified P insertion lying clearly within the validated deficiencies used in the verification analysis. Within this group, for a known number of total lines (transposition events), the number of genes mutated and how many times each was hit should have been determined with complete accuracy. Because the deficiencies included a majority of chromosome 2 and 3 genes (60.3 and 62.0%, respectively), and should be distributed effectively at random, this sample should accurately represent all insertions that cause a phenotype.

Focusing on the less-mutagenized chromosome first, we determined that 154 of the 535 third chromosome genes had been hit once, 43 twice, 16 three times, 6 four times, and 5 five times and that 18 were previously discussed hotspot loci hit six or more times (Table 1). Despite the small number of hotspot loci, they accounted for 204 of the 535 insertions (38%). First, we attempted to fit the data to a Poisson distribution, ignoring for the moment the obvious presence of hotspot genes. The best distribution ( = 0.558; Table 1) fit the data poorly because it predicted only 8.0 genes (instead of 16) hit three times, only 1.1 (instead of 6) hit four times, and 0.1 instead of 5 hit five times (² = 270, P << 0.001). To determine if the observed "excess" of genes hit three to five times was caused by the statistical tail from the hotspot loci, we used a binomial distribution to model their contribution (Table 1). The distribution used maximizes the contribution of hotspot genes to the classes of genes hit 3–5 times, while yielding the observed number of genes hit 6–12 times. Despite this, the results reveal that there are too few hotspot genes to account for the excess of genes hit 3–5 times (Table 1; ² = 20, P << 0.001).

Consequently, a class of genes of intermediate mutability must exist (warmspot genes). To estimate the size of this class, we fit the data for genes hit one to five times on the assumption of two mutability classes, warmspot and coldspot genes. Postulating 115 "warmspot" genes ( = 1.51) and 613 "coldspot" genes ( = 0.241) produced a good fit to the data (Table 1; ² = 0.81, P >> 0.05). Extrapolating the warmspot and coldspot data to the entire chromosome and adding the whole chromosome hotspot data, the following was predicted for the third chromosome: 27 hotspot loci + 115/0.603 = 191 warmspot loci + 613/0.603 = 1017 coldspot loci.

We next considered the second chromosome and found that 737 independent verified lines defined 190 genes that had been hit once, 57 twice, 19 three times, 17 four times, 5 five times, and 32 that were hotspot loci hit six or more times (Table 1). Hotspot insertions accounted for 288 of these lines (39%). Again, at least two general classes of mutability were required to fit the data from non-hotspot lines, even after correcting for the contribution of hotspot genes (Table 1; ² = 36, P << 0.001). Because we expected genes on the second and third chromosomes to have the same average mutabilities, we reasoned that the Poisson parameters for chromosome 2 warmspot and coldspot loci should correspond to parameters of the corresponding chromosome 3 genes corrected for the more extensive mutagenesis that was carried out on chromosome 2. The relative fraction of independent single-insert lines analyzed on chromosome 2 compared to chromosome 3 was 737/535 = 1.38. Multiplying the warmspot and coldspot class Poisson parameters determined for chromosome 3 by 1.38 gave the expected values on chromosome 2 ( = 2.08 and 0.331). Values of 110 warmspot and 680 coldspot loci on chromosome 2 were then determined to fit the distribution (Table 1; ² = 3.8, P >> 0.05). Thus, chromosome 2 is predicted to house 47 hotspot genes, 110/0.62 = 177 warmspot genes and 680/0.62 = 1097 coldspot genes.

	RESULTS

TOP ABSTRACT MATERIALS AND METHODS RESULTS DISCUSSION LITERATURE CITED

Rationale:
The gene disruption library was assembled from ~3900 starting lines that had been produced in seven separate single P-element mutagenesis screens (Table 2). Each starting line contained one (or a few) P-element insertion on an autosome bearing a newly induced scorable recessive phenotype. The process of going from this amalgamated raw collection to the finished library involved (1) localizing the insertions by in situ hybridization to polytene chromosomes at high resolution; (2) identifying strains with allelic insertions by inter se complementation crosses; (3) verifying that insertions were responsible for the mutant phenotype by crossing to chromosomes bearing deficiencies; and (4) sequencing DNA flanking the insertions and comparing it to EST and genomic sequence databases (SPRADLING et al. 1995 ). Single-insert-bearing strains that appear to disrupt distinct genes based on all these criteria constitute the final library, or "primary collection." Because of the requirement for complementation testing, the project was designed initially to focus on genes that mutate to a recognizable lethal, sterile, or visible phenotype.

Identifying single-insert lines:
The P insertion(s) in each line was cytogenetically localized by in situ hybridization as described previously (SPRADLING et al. 1995 ; see also MATERIALS AND METHODS). The number of lines localized from each screen is given in Table 2. Highly consistent and accurate localizations were required for the success of the complementation analysis. Images of each localization were digitized and stored (http://www.fruitfly.org/p_disrupt/). Based on these results, a significant number of strains were immediately eliminated from consideration for the primary collection. Two hundred seven lines were discarded because they did not represent independent insertions (see MATERIALS AND METHODS) and >900 lines were eliminated because they contained two or more insertions or a rearrangement on the mutation-bearing chromosome. A total of 2695 independently derived strains bearing single P-element insertions (1643 on II, 1052 on III) on intact chromosomes were retained. The P-element insertion site within each primary collection strain is listed in Table 4 and Table 5.

Identifying allelic mutations:
Complementation crosses were carried out inter se between lines whose insertions were located near each other (see MATERIALS AND METHODS). The maximum cytogenetic distance between the reported positions of insertions that is required to ensure they are not allelic depends critically on the accuracy of the in situ localization. We complementation tested lines when the distance between their elements was six to eight bands or less. This should have been sufficient to eliminate errors even in cytogenetically difficult regions, because the divergence in the reported positions of allelic insertions averaged less than one band (SPRADLING et al. 1995 ). The molecular analyses reported below provide further independent verification that allelic lines were not missed due to localization errors.

The complementation analysis provided considerable insight into the frequency with which individual loci are mutated by P elements (see Table 4 and Table 5). In particular, 74 complementation groups on the autosomes were identified that are hotspots for P-element insertion with between 6 and 37 alleles each. Because of the size of our data set, these loci likely comprisevirtually all the P-element insertion hotspots on the autosomes. Following completion of the complementation analysis, one allele of each complementation group was retained for the primary collection (see Table 2).

Verifying that the insertions cause mutations:
Three criteria were used to determine if the P-element insertion in a given single insert line was likely to be responsible for the observed mutant phenotype. First, if the mutation failed to complement one or more independently derived strains whose insertions had been localized nearby, then it was considered verified along with all the other insertions in the complementation group so defined. (The chance that such lines actually contained identical secondary or background mutations was negligible as indicated by test crosses with lines whose insertions were at different sites.) To apply the second verification test, the strain in question was crossed to deficiency chromosomes whose cytogenetically determined breakpoints (Table 3) indicated that they might lack the disrupted gene. Crosses were scored based on the presumed phenotype of the insertion (Table 4 and Table 5, "Df comp" and "Df noncomp"). Lines that failed to complement were considered to be verified, because the chance that a background mutation was closely linked to the P element was acceptably small. If complementation was observed, the line was discarded if its insertion clearly fell within the deficiency boundaries; otherwise it was retained but remained unverified. These two tests, combined with further verification based on the analysis of flanking DNA sequences as described below, allowed the total number of lines in the primary collection to be reduced to 1045, of which 725 (69%) are verified (see Table 2). Of these lines, 93% disrupt vital genes, while most of the remainder cause male or female sterility. The phenotype and verification status of each line are shown in Table 4 and Table 5.

We can estimate the approximate number of bogus lines that remain in the library. First, the overall fraction of verified lines arising from each screen is calculated by restricting our analysis to those lines whose insertions clearly fall within the boundaries of valid deficiencies and hence can be reliably tested (Table 2, "in Df"). This subgroup represents >60% of all the lines and should be representative of each screen as a whole. The proportion of lines that were verified ranges from 48–88% among the seven screens. Assuming that insertions falling outside the deficiencies are as likely to be valid as those inside allowed us to estimate the number of unverified primary collection lines from each starting screen that are likely to be valid. After making this final correction, the final number of different genes disrupted by P insertions in the collection is estimated to be 953 (Table 2). Using this information we also determined an overall efficiency for each of the seven screens, defined as the percentage of raw lines that contain a single insertion causing its associated phenotype (Table 2, "screen efficiency").

Deficiency chromosomes with accurate breakpoints are a valuable genetic resource. Knowledge of the true extent of material deleted in deficiency stocks was improved as a by-product of verifying the P insertions. The location of each verified insertion predicted the expected complementation behavior with relevant deficiencies. In cases where contradictions were observed, the breakpoints of the deficiency could sometimes be refined on the basis of the cytogenetic localizations of the terminal P elements (see Table 4 and Table 5). A number of such corrections have been incorporated into FlyBase (see flybase.bio.indiana.edu:80/.bin/fbabsq.html). Table 2 shows current estimates of the deficiency breakpoints used in these studies.

Characterizing insertions using flanking DNA sequence:
The genomic DNA sequence flanking the insertion sites in the primary collection lines was needed to complete the verification process and to begin associating lines with specific genes. Physically associating as many insertions as possible with specific sites in the genome would also enhance the usefulness of the primary collection for gene mapping and for directed mutational screening using accurately positioned starting strains (SPRADLING et al. 1995 ). Consequently, we attempted to recover genomic DNA adjacent to the 5', 3', or both sides of the P element from every remaining candidate primary collection line following completion of the genetic verification tests. Both plasmid rescue and inverse PCR were used. A single sequencing run was carried out beginning at the insertion site of all recovered flanks (see MATERIALS AND METHODS). Despite a shorter average amount of sequence recovered, inverse PCR was successful at a slightly higher average frequency (85% vs. 80%) and could be carried out in a 96-well format that allowed lines to be analyzed more rapidly. If both a 5' and 3' sequence was obtained, the two runs were merged in a single contig.

The sequences flanking the insertions were initially compared among themselves as an additional verification test. We wished to eliminate lines whose insertions were very close together but that behaved genetically like separate genes. Such lines are likely to be produced when chromosomes bearing nonallelic background mutations acquire insertions within the same nonvital gene. The genetic behavior of the resulting strains will cause them to survive into the primary collection if their insertions lie outside existing deficiencies. On the other hand, we did not want to eliminate valid insertions in adjacent genes. Consequently, in the absence of additional information, nonallelic insertions separated by 100 bp or more were assumed to represent distinct genes. When the separation was <100 bp, usually only one (if verified) or neither line was retained in the primary collection. Rarely, this might have led to the loss of valid lines, for example, in cases of overlapping genes or intragenic complementation, but it allowed us to discard nearly 100 questionable strains for the collection.

After completing these tests 1045 lines remained in the primary collection. Flanking sequence information has been obtained from 921 of the lines in this final group (88%). Accession numbers for each strain are listed in Table 4 and Table 5 ("Sequence"). These sequences, including the position of the insertion, are listed on the BDGP website (http://www.fruitfly.org/p_disrupt/).

Associating primary collection lines with genes:
The primary collection provides an opportunity to link ~1000 Drosophila genes with a genetic phenotype. Because these strains and genetic data have been publicly available from the inception of the project, the Drosophila research community has extensively utilized many lines from the primary collection (and the precursor raw collections). Publications describing at least 250 different Drosophila genes have employed strains from the collection (see Table 4 and Table 5, "References"). In many cases, the P-element disruption strain played a major role in the initial characterization of the gene in question.

To identify as many additional genes as possible the P-element flanks were searched against all Drosophila sequences in GenBank and ~26 Mb of genomic sequence (most searches are current as of December 1998). To test the accuracy of flanking sequence recovery, the polytene location of the P element in each of the 286 lines whose flanking sequences matched genomic sequence determined by BDGP was compared to the independently mapped polytene location of the corresponding P1 clones. Only a few discrepancies resulted, presumably due to the rare recovery of sequence from a cryptic P element, and in these cases a correct flanking sequence was sought. These searches provided a wide variety of valuable information. They confirmed most of the 250 published gene assignments, identified many additional characterized Drosophila genes disrupted by strains in the collection, and molecularly positioned the insertion sites within all these loci. Of the additional Drosophila genes, 55 had previously been characterized only at the molecular level (Table 6).

Further links to well-characterized genes were discovered by associating the insertions with Drosophila transcripts defined by EST sequencing. About 48,000 Drosophila EST sequences were available for these comparisons. A total of 376 insertions were located close to or within an EST sequence, usually near the 5' end (see Table 4 and Table 5). Mutation-causing P elements are known to preferentially cluster in the 5' region of the affected genes (see SPRADLING et al. 1995 ), a tendency that probably increases the chance of recovering overlaps between the short flanking sequences and 5' ESTs. For each line with a matching EST, the relevant "clot" (consensus sequence of overlapping ESTs) sequence was conceptually translated and used to search protein databases. These comparisons associated 76 more primary collection lines with previously undescribed Drosophila genes encoding proteins related to characterized genes from other species (Table 7). These new Drosophila genes have been named on the basis of the name of their ortholog. Genes are listed in Table 7 only if there is a strong match within the region of overlap and if a study of the ortholog's properties has been published. BDGP has determined complete complementary DNA (cDNA) sequences for some of these genes (Table 7). The approaches described so far linked 450 primary collection lines with known Drosophila genes or with orthologs of characterized genes in other organisms (Table 4 and Table 5).

Although the insertions in the remaining lines were not associated with a well-characterized gene or ortholog, it was still possible to link many of them with predicted transcripts and ORFs. The sequence comparisons associated the insertions in 135 additional lines with ESTs whose clots either predicted novel proteins or matched proteins conceptually encoded by ESTs or ORFs from other organisms. BLAST reports of these searches, including periodic updates, are available by searching the BDGP website using the appropriate EST (Table 4 and Table 5). Finally, the insertions within 138 of the remaining lines not associated with genes or ESTs were localized within sequenced portions of the Drosophila genome. Bioinformatic analyses of the sequences flanking these insertions reveal candidate ORFs, although such studies have not yet been carried out systematically. In sum, therefore, 706 of the 1045 primary collection strains (67%) already link known or candidate genes with mutant phenotypes. It should be possible to make most of the remaining gene-mutant associations by the time genome and EST sequencing nears completion.

P-element selectivity:
This study reveals the identity of most genes that are hotspots for P-element insertion on the autosomes (Table 4 and Table 5, "Alleles"). We searched for common properties that might explain their efficiency as P-element insertional targets. Hotspot genes are not associated with generally high transcription levels, because only 30% of the genes in the primary collection with more than five alleles have an associated EST sequence, compared to 36% for the collection as a whole. Hotspot genes might be those actively transcribed in premeiotic germline cells, where P elements usually transpose; however, the few genes in the collection whose transcripts are abundant in early germ cells, including vasa, bam, and hsp83, were each hit only once. Indeed, our comparisons uncovered no common biological features such as size, location, or regulation that might explain why hotspot genes are highly susceptible to P-element insertion.

We also considered whether strong preferences exist for insertion within certain classes of genes among all those disrupted in the collection. The primary collection includes an estimated 30% of readily mutable autosomal genes. Genes involved in signal transduction were usually well represented, because the collection mutates ~50% of all autosomal genes known to be involved in the EGFR, dpp, ras, wg, hh, or N signaling pathways. In addition, disruptions were obtained in 46% of autosomal posterior group genes, 31% of trithorax and Polycomb group genes, but only 14% of ribosomal protein genes. It remains unclear if these differences reflect more than the research priorities of the Drosophila research community.

Not all insertion sites were associated within protein-coding genes. One P element was located within a 5S rDNA repeat and four interrupted tRNA clusters. Nine lines, two of which disrupt the genes Distal-less and fruitless, were found by sequence analysis to contain insertions within the LTR sequence of a Drosophila retrotransposon related to the yoyo element of the Mediterranean fruit fly Ceratitis capitata (ZHOU and HAYMER 1997 ; see also FBgn0021759). The abundance of this element was low overall and all the insertions clustered in a small part of the LTR, a likely hotspot. Two other multicopy target sites were the telomere associated sequence (TAS) element, with six insertions, and the hoppel element, with one insertion. Both elements have been shown previously to be frequent targets of P-element insertion (KARPEN and SPRADLING 1992 ; ZHANG and SPRADLING 1995 ; D. STEWART and A. SPRADLING, personal communication). Because most insertions within repetitive sequences would not be expected to disrupt vital functions, these observations probably reflect which repetitive target sequences are frequently located within the introns or immediate flanks of vital genes in the strains used.

Modeling mutational saturation:
The gene disruption project provides a much larger and better-characterized data set than has been previously available for analyzing the site specificity of P-element transposition. This is an important question for determining the appropriate strategy to expand the collection. The insertional specificity of P elements must be extremely broad to achieve complete or nearly complete coverage of all Drosophila genes. In contrast, previous studies inferred that a significant percentage of Drosophila genes, perhaps as great as 50%, are refractory to mutation using P elements (see KIDWELL 1986 ; TOROK et al. 1993 ). If true, this would imply that a different method of mutagenesis is needed to complete the gene disruption project (SPRADLING et al. 1995 ). However, these conclusions remain highly uncertain, because previous studies of saturation behavior utilized raw collections of unverified lines that differ in P-element content and did not correct for locus-specific differences in mutagenesis rates. The total number of different genes mutagenized clearly rises more slowly than expected by assuming that nearly all genes are equally susceptible to P-element insertion. However, this observation alone cannot distinguish between the presence of genes refractory to P-element insertion and the presence of gene classes that differ significantly in P-element mutability. Fortunately, the very information gathered to build the primary collection also allows one to more accurately deduce the saturation behavior of P elements.

We focused on the large subset of the P-element lines from the collections whose insertions lie within the boundaries of validated deficiencies. Within this group, for a known number of total lines (transposition events), the number of genes mutated and how many times each was hit has been determined with complete accuracy. Because the deficiencies included a majority of chromosome 2 and 3 genes (60.3 and 62.0%, respectively), and should be distributed effectively at random, this sample should accurately represent all insertions that cause a phenotype. When we analyzed the distribution of insertional mutations among this set of genes, it was clear that the data did not fit a simple Poisson distribution (see MATERIALS AND METHODS; Table 1). The most obvious problem was the hotspot loci. On chromosomes 2 and 3, just 18 or 32 loci account for 38 or 39% of all insertions, respectively. However, even after subtracting the contribution of these hotspot loci, the distribution of gene mutabilities remained skewed (see MATERIALS AND METHODS; Table 1). Consequently, a class of warmspot genes was inferred whose mutability is intermediate between the hotspot loci and the large group of low mutability coldspot genes. Assuming the existence of three major mutability classes allowed a good fit to the data.

This model provides several useful insights into P-element behavior. The third chromosome is predicted to contain 27 hotspot loci + 191 warmspot loci + 1017 coldspot loci, while the second chromosome should house 47 hotspot genes + 177 warmspot genes + 1097 coldspot genes. Despite accounting for only 17% of all genes, the 368 warmspot and 74 hotspot genes account for ~70% of all transposition events. As a result, virtually all the hotspot loci and 80–90% of the warmspot loci have already been defined by strains in the primary collection. On the other hand, only 22–28% of the coldspot loci have so far been disrupted. However, assuming that there are 1400 vital loci per major autosome (MIKLOS and RUBIN 1996 ), and considering that 93% of the disruptions in our collection are of vital genes, then the model predicts that at least 2556 x 0.93/2800 = 85% of vital genes can eventually be mutated using P elements. Thus, the existence of the hotspot and warmspot genes is the reason that mutational saturation proceeds more slowly than expected on the basis of a single class Poisson analysis, but the final level of saturation is higher than previously appreciated. Indeed, if gene mutabilities actually vary more broadly than three discrete classes, as seems likely, the true level of saturation will exceed 85%. There is no reason to suspect that P-element insertional preferences differ between vital and nonvital genes, so the conclusions drawn here should apply to Drosophila genes generally. These results suggest that a much larger fraction of Drosophila genes than previously supposed, at least 85% and possibly 100%, are susceptible to inactivation by P-element insertion.

	DISCUSSION

TOP ABSTRACT MATERIALS AND METHODS RESULTS DISCUSSION LITERATURE CITED

Collections of gene disruptions as tools for functional genomics:
It is now possible in theory to mutate virtually any gene that has been molecularly identified in the major multicellular model organisms and to isolate the mutant allele on a standard genetic background free of secondary lesions. In practice, obtaining mutants remains a time-consuming task that constitutes the largest current impediment to progress in understanding gene function in vivo. While it has become widely accepted that gene sequence and structure can be more efficiently analyzed on a genome-wide scale, a similar consensus on the value of whole genome gene disruption has been slow to develop. As a result, linking genes with mutations remains a cottage industry pursued by individual laboratories. The work reported here has been motivated by the belief that complete gene mutation libraries are feasible and have the potential to greatly accelerate the rate at which gene function can be analyzed. We feel that whole genome mutant collections belong together with complete genome and cDNA sequences as essential tools for future biological research.

The BDGP gene disruption library represents a significant step toward the ultimate goal of stockpiling an identified mutation in every Drosophila transcription unit. The current collection of single P-element insertions provides a particularly useful type of link between the genetic and molecular properties of ~1000 different autosomal genes that can mutate to a readily recognizable phenotype. This is more than the number of genes that have been characterized at both the genetic and molecular levels in any of the other widely used model multicellular eukaryotes, including Arabadopsis, C. elegans, zebrafish, or mice, and exceeds the number of gene-mutation links known in humans. As a reflection of its utility, lines from the BDGP collection have been utilized in publications characterizing more than 250 different genes since 1988 (Table 4 and Table 5).

Expanding the collection:
Because the Drosophila genome is believed to house ~12,000 genes (MIKLOS and RUBIN 1996 ), the current primary collection is still far from complete. Two basic approaches can be considered for expanding its coverage. A targeted strategy would avoid reisolating new mutations in genes that have already been disrupted in the existing collection or by individual Drosophila researchers. A general strategy for identifying mutations in any gene encoding a protein that can be detected with a specific antiserum has been developed (DOLPH et al. 1992 ). However, a substantial number of genes that express proteins only at low levels may be refractory to disruption by this approach. Consequently, continuing the insertional mutagenesis strategy used previously in some form appears to be the most promising approach to completing the collection.

Significant improvements are possible in the short term by incorporating several new collections of insertions that have already been constructed since the project was initiated (ERDELYI et al. 1995 ; DEAK et al. 1997 ; RORTH et al. 1998 ). The third chromosome collection described by DEAK et al. 1997 is similar in size to the collection of TOROK et al. 1993 on chromosome 2, but preliminary estimates by the authors indicate a higher screen efficiency. Incorporating these lines into the existing collection should increase the number of third chromosome lines to >600 and equalize the saturation levels of the two major autosomes.

It will also be of value to carry out new mutagenesis screens. A major variable in the generation of single P-element-induced mutations is the wide variation in screen efficiency that is documented here (Table 2). One factor that can affect screen efficiency is the overall rate of P transposition. High transposition rates like those in the screen of TOROK et al. 1993 produce an excess of lines with more than one P-element insertion (>23% in this case). High transposition rates probably also cause secondary mutations as elements transpose and excise at multiple sites over several germ cell division cycles. However, our results imply that the rate of transposition and amount of secondary damage are not always correlated and are not simply a function of the P elements used (Table 2). Both BIER et al. 1989 and TOROK et al. 1993 employed the PlacW and 2-3 P elements but obtained very different frequencies of multiple insert lines, rates of background mutation, and overall screen efficiencies. In contrast, the screen of COOLEY et al. 1988 using PUChsneo and a weak mobilizing P element exhibited a low transposition rate but still gave an efficiency of only ~50%. Consequently, our results suggest that currently unidentified factors in the genetic backgrounds used for P-element mutagenesis affect the prevalence of damage at chromosomal sites that do not retain P-element sequences. Unfortunately, the nature of these factors remains poorly understood.

The number of new lines that needs to be characterized to substantially complete the gene disruption project can be estimated from our analysis of saturation. The genome contains ~3600 vital genes, at least 3100 of which fall into the coldspot class. Statistically, twice this number of insertions, 6200, must be recovered in this class of genes to achieve 87% saturation. Because only 30% of raw insertions target the coldspot class, and because the best screens produce only 85% verified single insert lines, achieving 87% saturation would require the isolation and analysis of 6200/(0.3 x 0.85) = 24,300 autosomal insertions associated with phenotypes. This represents about six times as many lines as were analyzed in the current project.

A molecular strategy for finishing the mutation library:
Even a project of this size is feasible, although a very large effort would be required. However, a continuation of the current approach would not address the estimated two-thirds of all genes that do not mutate to a readily detectable phenotype in genetic screens. To obtain P-element insertions that disrupt such genes, it will be necessary to look directly for changes in their structure. With large amounts of genomic and EST sequences becoming available and a strong commitment to completing the Drosophila genome sequence within 1–3 years (COLLINS et al. 1998 ; VENTER et al. 1998 ), a strategy based entirely on molecular mapping is becoming feasible. A new generation of P-element misexpression vectors (RORTH 1996 ) are attractive candidates for use with this approach. These insertions not only can disrupt genes but also are frequently able to program the controlled misexpression of the affected protein. This option should accelerate the collection of functional information, especially on the many genes whose loss does not produce an immediately recognizable phenotype.

We propose to inaugurate a phase two gene disruption project whose goal would be to disrupt all Drosophila genes, regardless of phenotype. Flanking DNA will be recovered from a large number of raw insertion lines and sequenced, much as was done with the primary collection lines in the current collection. The short sequences obtained will allow most new insertions to be precisely positioned on the genomic sequence. Consulting EST and cDNA sequences, gene predictions, ORF homologies, and other relevant data in the vicinity of the insertion sites will allow rapid predictions as to whether each new insertion is likely to disrupt or misexpress an ORF not currently represented in the collection. Lines that do not appear to do so would be quickly discarded. Recently, this strategy has received a valuable test within the fully sequenced 2.9-Mb Adh region (ASHBURNER et al. 1999 ). By mapping all available P elements onto the genomic DNA sequence, not just those causing phenotypes as described here, the number of gene-mutation links was increased substantially (see Table 4).

The phase two strategy has several distinct advantages. First, it broadens the project to include all Drosophila genes. In addition, it greatly simplifies the work required to characterize new candidate lines, compensating in part for the much larger number of lines that will need to be analyzed. Polytene localizations are unnecessary, because multiinsert lines can be detected through their production of more than one distinct P-element flanking sequence. Balancing most of the newly mutagenized chromosomes is not required. Genetic complementation is not necessary, because redundant lines can increasingly be identified on the basis of their location. However, there are several requirements for success. First, the Drosophila genome sequence must be completed in a timely manner. Second, semiautomated methods for recovering and sequencing flanking DNA segments must be further improved. Finally, bioinformatic tools to assist decision making about line retention must be developed.

We can calculate the approximate number of lines that will need to be analyzed during the phase two project. About 11,000 of the estimated 12,000 Drosophila genes are predicted to fall into the coldspot class, assuming that the P-element mutability of all genes is similar to that of vital genes. Therefore, if 30% of new insertions fall in the coldspot class as in the case with lethal insertions, and 95% of raw lines contain only one insertion, then 2 x 11,000/(0.3 x 0.95) = 77,000 lines would be required for 87% saturation. However, two observations suggest that some unselected insertions will fail to disrupt any gene, increasing the total number of lines that will need to be analyzed. First, P elements are attracted to at least some repetitive sequences such as yoyo, TAS, and hoppel, which are often located at nonmutagenic sites within the genome. The fraction of insertions that land in such sites might be significant. Second, P insertions that cause phenotypes cluster around the 5' region of genes (SPRADLING et al. 1995 ; data not shown). Previously, insertions located too far upstream from transcription start sites, or at nonmutagenic sites within large introns, have been edited out by the requirement for a phenotypic effect. In phase two, they would be recovered and analyzed, lowering efficiency.

The relative fraction of unselected insertions that disrupt genes can be estimated, however. If all insertions mutated genes, then 33% of new transpositions should cause a recognizable phenotype, because about one-third of genes are thought to mutate in this manner. Instead, only ~15% of raw insertions recovered on clean chromosomes cause a recognizable phenotype (see citations in Table 2). Consequently, as many as 77,000/0.5 = 154,000 insertions might need to be screened to obtain 87% saturation across all Drosophila genes. However, in practice, this may be an overestimate. P elements can be excised imprecisely to generate deletions adjacent to the insertion site. Because of the large number of mapped insertions that will be available by the time phase two is only partially complete, a strategy in which some genes are disrupted by excising nearby nonmutagenic insertions might substantially reduce the final number of strains that need to be generated and analyzed.

A gene disruption library represents a fundamental and indispensable resource for analyzing gene function on a genome-wide scale. The BDGP gene disruption project has already accelerated studies of Drosophila gene function and is likely to be even more valuable as coverage increases. A pilot screen for phase two has already been completed in collaboration with several laboratories (RORTH et al. 1998 ). A total of 2400 lines from this project have been mapped and initially analyzed (BDGP, unpublished results; see http://www.fruitfly.org/bfd/). We believe that researchers using Drosophila (and other model multicellular organisms) are rapidly approaching an era where obtaining mutations, the basic tools for understanding gene function in vivo, will no longer limit the progress of research.

	ACKNOWLEDGMENTS

BDGP acknowledges all those researchers who participated in constructing the strains that were used in this project. These include L. Ackerman, M. Alvarado, S. Barbel, C. Berg, E. Bier, S. Bockheim, M. Boedingheimer, R. Carretto, Z. Chang, L. Cooley, M. Fuller, U. Gaul, R. Glaser, E. Grell, B. Harkins, M. Heck, L. Higgins, L. Jan, Y.-N. Jan, G. Karpen, R. Kelley, I. Kiss, A. Laughon, K. Lee, L. Lee, G. Mardon, K. McCall, D. McKearin, C. Montell, D. Montell, T. Overbode, B. Price, J. Riesgo, M. Scott, S. Shepherd, R. Smith, D. Thompson, T. Tick, T. Törok, J. Tower, T. Uemura, H. Vassin, E. Verheyen, S. Wasserman, and L. Yue. We are also grateful to many workers who in the course of this study communicated complementation results and other information on specific P-element strains. In particular, John Roote and Paul Lasko shared complementation data for 2L divisions 24-36 and 37-38. H. Bellen (various), Erica Roulier (29A), Ken Howard (45), Jordan Raff (46A), Elliott Goldstein (46), Robert Burgess (47EF), Claire Russell (49EF), Paul Wes (52E), and Boris Dunkov (99F) contributed and confirmed results in the cytogenetic regions indicated. We thank A. deGrey for assistance in analyzing chromosome 2 data. This work was supported by a genome center grant (P50NIHHG750) from the National Institutes of Health. A.C.S. and G.M.R. are Howard Hughes Medical Institute Investigators.

Manuscript received January 29, 1999; Accepted for publication April 26, 1999.

	LITERATURE CITED

TOP ABSTRACT MATERIALS AND METHODS RESULTS DISCUSSION LITERATURE CITED

ALLENDE, M. L., A. AMSTERDAM, T. BECKER, K. KAWAKAMI, and H. GAIANOAND et al., 1996  Insertional mutagenesis in zebrafish identifies two novel genes, pescadillo and dead eye, essential for embryonic development. Genes Dev. 10:3141-3155[Abstract/Free Full Text].

ALSINA, B., F. SERRAS, J. BAGUNA, and M. COROMINAS, 1998  patufet, the gene encoding the Drosophila melanogaster homologue of selenophosphate synthetase, is involved in imaginal disc morphogenesis. Mol. Gen. Genet. 257:113-123[Medline].

ANDREW, D. J., A. BAIG, P. BHANOT, S. M. SMOLIK, and K. D. HENDERSON, 1997  The Drosophila dCREB-A gene is required for dorsal/ventral patterning of the larval cuticle. Development 124:181-193[Abstract].

ARORA, K., H. DAI, S. G. KAZUKO, J. JAMAL, and M. B. O'CONNOR et al., 1995  The Drosophila schnurri gene acts in the Dpp/TGF-beta signaling pathway and encodes a transcription factor homologous to the human MBP family. Cell 81:781-790[Medline].

ASHBURNER, M., 1990 Drosophila: A Laboratory Manual. Cold Spring Harbor Laboraory Press, Cold Spring Harbor, NY.

ASHBURNER, M., S. MISRA, J. ROOTE, S. LEWIS, and R. BLAZEJ et al., 1999  An exploration of the sequence of a 2.9-Mb region of the genome of Drosophila melanogaster: the Adh region. Genetics 153:179-219[Abstract/Free Full Text].

BARRETT, K., M. LEPTIN, and J. SETTLEMAN, 1997  The Rho GTPase and a putative RhoGEF mediate a signaling pathway for the cell shape changes in Drosophila gastrulation. Cell 91:905-915[Medline].

BAUMGARTNER, S., D. MARTIN, C. HAGIOS, and R. CHIQUET-EHRISMANN, 1994  Ten-m, a Drosophila gene related to tenascin, is a new pair-rule gene. EMBO J. 13:3728-3740[Medline].

BAUMGARTNER, S., D. MARTIN, R. CHIQUET-EHRISMANN, J. SUTTON, and A. DESAI et al., 1995  The HEM proteins: a novel family of tissue-specific transmembrane proteins expressed from invertebrates through mammals with an essential function in oogenesis. J. Mol. Biol. 251:41-49[Medline].

BAUMGARTNER, S., J. T. LITTLETON, K. BROADIE, M. A. BHAT, and R. HARBECKE et al., 1996  A Drosophila neurexin is required for septate junction and blood-nerve barrier formation and function. Cell 87:1059-1068[Medline].

BEGEMANN, G., A. M. MICHON, L. VAN DER VOORN, R. WEPF, and M. MLODZIK, 1995  The Drosophila orphan nuclear receptor Seven-up requires the Ras pathway for its function in photoreceptor determination. Development 121:225-235[Abstract].

BELLAICHE, Y., I. THE, and N. PERRIMON, 1998  Tout-velu is a Drosophila homologue of the putative tumour suppressor EXT-1 and is needed for Hh diffusion. Nature 394:85-88[Medline].

BELLEN, H. J., C. J. O'KANE, C. WILSON, U. GROSSNIKLAUS, and R. K. PEARSON et al., 1989  P-element-mediated enhancer detection: a versatile method to study development in Drosophila. Genes Dev. 3:1288-1300[Abstract/Free Full Text].

BERG, C. and A. SPRADLING, 1991  Studies on the rate and site-specificity of P element transposition. Genetics 127:515-524[Abstract].

BHAT, M. A., A. V. PHILP, D. M. GLOVER, and J. BELLEN, 1996  Chromatid segregation at anaphase requires the barren product, a novel chromosome-associated protein that interacts with Topoisomerase II. Cell 87:1103-1114[Medline].

BHATT, A. M., T. PAGE, E. J. LAWSON, C. LISTER, and C. DEAN, 1996  Use of Ac as an insertional mutagen in Arabidopsis. Plant J. 9:935-945[Medline].

BIER, E., H. VASSIN, S. SHEPHERD, K. LEE, and K. MCCALL et al., 1989  Searching for pattern and mutation in the Drosophila genome with a P-lacZ vector. Genes Dev. 3:1273-1287[Abstract/Free Full Text].

BOULIANNE, G. L., A. DE LA CONCHA, J. A. CAMPOS-ORTEGA, L. Y. JAN, and Y. N. JAN, 1991  The Drosophila neurogenic gene neuralized encodes a novel protein and is expressed in precursors of larval and adult neurons. EMBO J. 10:2975-2983[Medline].

BRAUN, A., J. A. HOFFMANN, and M. MEISTER, 1997  Drosophila immunity: analysis of larval hemocytes by P-element-mediated enhancer trap. Genetics 147:623-634[Abstract].

BRUMMEL, T., S. ABDOLLAH, T. E. HAERRY, M. J. SHIMELL, J. MERRIAM, L. RAFTERY, J. L. WRANA, and M. B. O'CONNOR, 1999  The Drosophila activin receptor baboon signals through dSmad2 and controls cell proliferation but not patterning during larval development. Genes Dev. 13:98-111[Abstract/Free Full Text].

BURNS, N., B. GRIMWADE, P. B. ROSS-MACDONALD, E. Y. CHOI, and K. FINBERG et al., 1994  Large-scale analysis of gene expression, protein localization, and gene disruption in Saccharomyces cerevisiae.. Genes Dev. 8:1087-1105[Abstract/Free Full Text].

CAMPBELL, G., H. GORING, T. LIN, E. P. SPANA, and S. ANDERSON et al., 1994  RK2, a glial-specific homeodomain protein required for embryonic nerve cord condensation and viability in Drosophila. Development 120:2957-2966[Abstract].

CAMPBELL, S. D., F. SPRENGER, B. A. EDGAR, and P. H. O'FARRELL, 1995  Drosophila Wee1 kinase rescues fission yeast from mitotic catastrophe and phosphorylates Drosophila Cdc2 in vitro. Mol. Biol. Cell 6:1333-1347[Abstract].

CASTRILLON, D. H., P. GONCZY, R. RAWSON, C. G. EBERHART, and S. VISWANATHAN et al., 1993  Toward a molecular genetic analysis of spermatogenesis in Drosophila melanogaster: characterization of male-sterile mutants generated by single P element mutagenesis. Genetics 135:489-505[Abstract].

CHANG, H. C. and G. M. RUBIN, 1997  14-3-3 epsilon positively regulates Ras-mediated signaling in Drosophila. Genes Dev. 11:1132-1139[Abstract/Free Full Text].

CHANG, Z., B. D. PRICE, S. BOCKHEIM, M. J. BOEDIGHEIMER, and R. SMITH et al., 1993  Molecular and genetic characterization of the Drosophila tartan gene. Dev. Biol. 160:315-332[Medline].

CLARK, K. A. and D. M. MCKEARIN, 1996  The Drosophila stonewall gene encodes a putative transcription factor essential for germ cell development. Development 122:937-950[Abstract].

COLLINS, F. S., A. PATRINOS, E. JORDAN, A. CHAKRAVARTI, and R. GESTELAND et al., 1998  New goals for the U.S. human genome project: 1998–2003. Science 282:682-689[Abstract/Free Full Text].

COOLEY, L., R. KELLEY, and A. C. SPRADLING, 1988  Insertional mutagenesis of the Drosophila genome with single P elements. Science 239:1121-1128[Abstract/Free Full Text].

COOLEY, L., E. VERHEYEN, and K. AYERS, 1992  chickadee encodes a profilin required for intercellular cytoplasm transport during Drosophila oogenesis. Cell 69:173-184[Medline].

CUI, X. and C. Q. DOE, 1992  ming is expressed in neuroblast sublineages and regulates gene expression in the Drosophila central nervous system. Development 116:943-952[Abstract].

DAVIES, S. A., S. F. GOODWIN, D. C. KELLY, Z. WANG, and M. A. SOZEN et al., 1996  Analysis and inactivation of vha55, the gene encoding the vacuolar ATPase B-subunit in Drosophila melanogaster reveals a larval lethal phenotype. J. Biol. Chem. 271:30677-30684[Abstract/Free Full Text].

D'AVINO, P. P. and C. S. THUMMEL, 1998  crooked legs encodes a family of zinc finger proteins required for leg morphogenesis and ecdysone-regulated gene expression during Drosophila metamorphosis. Development 125:1733-1745[Abstract].

DEAK, P., M. M. OMAR, R. D. SAUNDERS, M. PAL, and O. KOMONYI et al., 1997  P-element insertion alleles of essential genes on the third chromosome of Drosophila melanogaster: correlation of physical and cytogenetic maps in chromosomal region 86E-87F. Genetics 147:1697-1722[Abstract].

DEMAKOV, S. A., V. F. SEMESHIN, and I. F. ZHIMULEV, 1993  Cloning and molecular genetic analysis of Drosophila melanogaster interband DNA. Mol. Gen. Genet. 238:437-443[Medline].

DE NOOIJ, J. C., M. A. LETENDRE, and I. K. HARIHARAN, 1996  A cyclin-dependent kinase inhibitor, dacapo, is necessary for timely exit from the cell cycle during Drosophila embryogenesis. Cell 87:1237-1247[Medline].

DINGWALL, A. K., S. J. BEEK, C. M. MCCALLUM, J. W. TAMKUN, and G. V. KALPANA et al., 1995  The Drosophila snr1 and brm proteins are related to yeast SWI/SNF proteins and are components of a large protein complex. Mol. Biol. Cell 6:777-791[Abstract].

DOLPH, P. J., R. RANGANATHAN, N. J. COLLEY, R. W. HARDY, and M. SOCOLICH et al., 1992  Arrestin function in inactivation of G protein-coupled receptor rhodopsin in vivo. Science 260:1910-1916.

DONG, X., K. H. ZAVITZ, B. J. THOMAS, M. LIN, and S. CAMPBELL et al., 1997  Control of G1 in the developing Drosophila eye: rca1 regulates Cyclin A.. Genes Dev. 11:94-105[Abstract/Free Full Text].

DORN, R., J. SZIDONYA, G. KORGE, M. SEHNERT, and H. TAUBERT et al., 1993  Transposon-induced dominant enhancer mutations of position-effect variegation in Drosophila melanogaster.. Genetics 133:279-290[Abstract].

DUMAN-SCHEEL, M., X. LI, I. ORLOV, M. NOLL, and N. H. PATEL, 1997  Genetic separation of the neural and cuticular patterning functions of gooseberry.. Development 124:2855-2865[Abstract].

DURONIO, R. J., P. H. O'FARRELL, J. E. XIE, A. BROOK, and N. DYSON, 1995  The transcription factor E2F is required for S phase during Drosophila embryogenesis. Genes Dev. 9:1445-1455[Abstract/Free Full Text].

EBERHART, C. G. and S. A. WASSERMAN, 1995  The pelota locus encodes a protein required for meiotic cell division: an analysis of G2/M arrest in Drosophila spermatogenesis. Development 121:3477-3486[Abstract].

EBERHART, C. G., J. Z. MAINES, and S. A. WASSERMAN, 1996  Meiotic cell cycle requirement for a fly homologue of human Deleted in Azoospermia. Nature 381:783-785[Medline].

EDGAR, B. A. and P. H. O'FARRELL, 1989  Genetic control of cell divisions patterns in the Drosophila embryo. Cell 57:177-187[Medline].

ELDON, E., S. KOOYER, D. D'EVELYN, M. DUNMAN, and P. LAWINGER et al., 1994  The Drosophila 18-wheeler is required for morphogenesis and has striking similarities to Toll.. Development 120:885-899[Abstract].

ENDO, K., T. AKIYAMA, S. KOBAYASHI, and M. OKADA, 1996  Degenerative spermatocyte, a novel gene encoding a transmembrane protein required for the initiation of meiosis in Drosophila spermatogenesis. Mol. Gen. Genet. 253:157-165[Medline].

ERDELYI, M., A. M. MICHON, A. GUICHET, J. B. GLOTZER, and A. EPHRUSSI, 1995  Requirement for Drosophila cytoplasmic tropomyosin in oskar mRNA localization. Nature 377:524-527[Medline].

EULENBERG, K. G. and R. SCHUH, 1997  The tracheae defective gene encodes a bZIP protein that controls tracheal cell movement during Drosophila embryogenesis. EMBO J. 16:7156-7165[Medline].

FENG, Y., L. HUYNH, K. TAKEYASU, and D. M. FAMBROUGH, 1997  The Drosophila Na,K-ATPase alpha-subunit gene: gene structure, promoter function and analysis of a cold-sensitive recessive-lethal mutation. Genes Funct. 1:99-117[Medline].

FERNANDEZ, R., D. TABARINI, N. AZPIAZU, and M. FRASCH, 1995  The Drosophila insulin receptor homolog: a gene essential for embryonic development encodes two receptor isoforms with different signaling potential. EMBO J. 14:3373-3384[Medline].

FLETCHER, J. C. and C. S. THUMMEL, 1995  The Drosophila E74 gene is required for the proper stage- and tissue-specific transcription of ecdysone-regulated genes at the onset of metamorphosis. Development 121:1411-1421[Abstract].

FORBES, A. J., A. C. SPRADLING, P. W. INGHAM, and H. LIN, 1996  The role of segment polarity genes during early oogenesis in Drosophila. Development 122:3283-3294[Abstract].

FORJANIC, J. P., C. K. CHEN, H. JACKLE, and M. GONZALEZ-GAITAN, 1997  Genetic analysis of stomatogastric nervous system development in Drosophila using enhancer trap lines. Dev. Biol. 186:139-154[Medline].

FREEMAN, M., C. KLAMBT, C. S. GOODMAN, and G. M. RUBIN, 1992  The argos gene encodes a diffusible factor that regulates cell fate decisions in the Drosophila eye. Cell 69:963-975[Medline].

FROMMER, G., G. VORBRUGGEN, G. PASCA, H. JAECKLE, and T. VOLK, 1996  Epidermal egr-like zinc finger protein of Drosophila participates in myotube guidance. EMBO J. 15:1642-1649[Medline].

GAIANO, N., A. AMSTERDAM, K. KAWAKAMI, M. ALLENDE, and T. BECKER et al., 1996  Insertional mutagenesis and rapid cloning of essential genes in zebrafish. Nature 383:829-832[Medline].

GARRAWAY, L. A., L. R. TOSI, Y. WANG, J. B. MOORE, and D. E. DOBSON et al., 1997  Insertional mutagenesis by a modified in vitro Ty1 transposition system. Gene 198:27-35[Medline].

GARRITY, P. A., Y. RAO, I. SALECKER, J. MCGLADE, and T. PAWSON et al., 1996  Drosophila photoreceptor axon guidance and targeting requires the dreadlocks SH2/SH3 adapter protein. Cell 85:639-650[Medline].

GAUL, U., G. MARDON, and G. M. RUBIN, 1992  A putative Ras GTPase activating protein acts as a negative regulator of signaling by the Sevenless receptor tyrosine kinase. Cell 68:1007-1019[Medline].

GELLON, G., K. W. HARDING, N. MCGINNIS, M. M. MARTIN, and W. MCGINNIS, 1997  A genetic screen for modifiers of Deformed homeotic function identifies novel genes required for head development. Development 124:3321-3331[Abstract].

GEORGE, H. and R. TERRACOL, 1997  The vrille gene of Drosophila is a maternal enhancer of decapentaplegic and encodes a new member of the bZIP family of transcription factors. Genetics 146:1345-1363[Abstract].

GIGLIOTTI, S., G. CALLAINI, S. ANDONE, M. G. RIPARBELLI, and R. PERRNAS-ALONSO et al., 1998  Nup154, a new Drosophila gene essential for male and female gametogenesis is related to the nup155 vertebrate nucleoporin gene. J. Cell Biol. 142:1195-1207[Abstract/Free Full Text].

GILLESPIE, D. E. and C. A. BERG, 1995  Homeless is required for RNA localization in Drosophila oogenesis and encodes a new member of the DE-H family of RNA-dependent ATPases. Genes Dev. 9:2495-2508[Abstract/Free Full Text].

GONZALEZ-GAITAN, M. and H. JACKLE, 1997  Role of Drosophila alpha-adaptin in presynaptic vesicle recycling. Cell 88:767-776[Medline].

GOSSLER, A., A. L. JOYNER, J. ROSSANT, and W. C. SKARNES, 1989  Mouse embryonic stem cells and reported constructs to detect developmentally regulated genes. Science 244:463-465[Abstract/Free Full Text].

GOTO, S. and S. HAYASHI, 1997  Specification of the embryonic limb primordium by graded activity of Decapentaplegic. Development 124:125-132[Abstract].

GRETHER, M. E., J. M. ABRAMS, J. AGAPITE, K. WHITE, and H. STELLER, 1995  The head involution defective gene of Drosophila melanogaster functions in programmed cell death. Genes Dev. 9:1694-1708[Abstract/Free Full Text].

GUILLEMIN, K., J. GROPPE, K. DUCKER, R. TREISMAN, and E. HAFEN et al., 1996  The pruned gene encodes the Drosophila serum response factor and regulates cytoplasmic outgrowth during terminal branching of the tracheal system. Development 122:1353-1362[Abstract].

HACKER, U., X. LIN, and N. PERRIMON, 1997  The Drosophila sugarless gene modulates Wingless signaling and encodes an enzyme involved in polysaccharide biosynthesis. Development 124:3565-3573[Abstract].

HAHN, M. and H. JACKLE, 1996  Drosophila goosecoid participates in neural development but not in body axis formation. EMBO J. 15:3077-3084[Medline].

HAMILTON, B. A., M. J. PALAZZOLO, J. H. CHANG, K. VIJAYRAGHAVAN, and C. A. MAYEDA et al., 1991  Large scale screen for transposon insertions into cloned genes. Proc. Natl. Acad. Sci. USA 88:2731-2735[Abstract/Free Full Text].

HARVIE, P. D., M. FILIPPOVA, and P. J. BRYANT, 1998  Genes expressed in the ring gland, the major endocrine organ of Drosophila melanogaster.. Genetics 149:217-231[Abstract/Free Full Text].

HASSAN, B. A., S. N. PROKOPENKO, S. BREUER, B. ZHANG, and A. PAULULAT et al., 1998  skittles, a Drosophila phosphatidylinositol 4-phosphate 5-kinase, is required for cell viability, germline development and bristle morphology, but not for neurotransmitter release. Genetics 150:1527-1537[Abstract/Free Full Text].

HAY, B. A., D. A. WASSARMAN, and G. M. RUBIN, 1995  Drosophila homologs of baculovirus inhibitor of apoptosis proteins function to block cell death. Cell 83:1253-1262[Medline].

HEBERLEIN, U., T. WOLFF, and G. M. RUBIN, 1993  The TGFbeta homolog dpp and the segment polarity gene hedgehog are required for propagation of a morphogenetic wave in the Drosophila retina. Cell 75:913-926[Medline].

HECK, M. M. S., A. PEREIRA, P. PESAVENTO, Y. YANNONI, and A. C. SPRADLING et al., 1993  The kinesin-like protein KLP61F is essential for mitosis in Drosophila. J. Cell Biol. 123:665-679[Abstract/Free Full Text].

HONG, C. C. and C. HASHIMOTO, 1995  An unusual mosaic protein with a protease domain, encoded by the nudel gene, is involved in defining embryonic dorsoventral polarity in Drosophila. Cell 82:785-794[Medline].

HOROWITZ, H. and C. A. BERG, 1996  The Drosophila pipsqueak gene encodes a nuclear BTB-domain-containing protein required early in oogenesis. Development 122:1859-1871[Abstract].

HOSHIZAKI, D. K., 1994  Kruppel expression during postembryonic development of Drosophila. Dev. Biol. 163:133-140[Medline].

HOU, X. S., M. B. MELNICK, and N. PERRIMON, 1996  marelle acts downstream of the Drosophila HOP/JAK kinase and encodes a protein similar to the mammalian STATs. Cell 84:411-419[Medline].

ILIOPOULOS, I., I. TOROK, and B. M. MECHLER, 1997  The DnaJ60 gene of Drosophila melanogaster encodes a new member of the DnaJ family of proteins. Biol. Chem. Hoppe-Seyler 378:1177-1181.

ISAAC, D. D. and D. J. ANDREW, 1996  Tubulogenesis in Drosophila: a requirement for the trachealess gene product. Genes Dev. 10:103-117[Abstract/Free Full Text].

ITO, H., K. FUJITANI, K. USUI, K. SHIMIZU-NISHIKAWA, and S. TANAKA et al., 1996  Sexual orientation in Drosophila is altered by the satori mutation in the sex-determination gene fruitless that encodes a zinc finger protein with a BTB domain. Proc. Natl. Acad. Sci. USA 93:9687-9692[Abstract/Free Full Text].

JAENISCH, R., 1988  Transgenic animals. Science 240:1468-1474[Abstract/Free Full Text].

JIANG, J. and G. STRUHL, 1998  Regulation of Hedgehog and Wingless signalling pathways by the F-box/WD40-repeat protein slimb. Nature 391:493-496[Medline].

JUSTICE, R. W., O. ZILIAN, D. F. WOODS, M. NOLL, and P. J. BRYANT, 1995  The Drosophila tumor suppressor gene warts encodes a homolog of human myotonic dystrophy kinase and is required for the control of cell shape and proliferation. Genes Dev. 9:534-546[Abstract/Free Full Text].

KANIA, A., A. SALZBERG, M. BHAT, D. D'EVELYN, and Y. HE et al., 1995  P-element mutations affecting embryonic peripheral nervous system development in Drosophila melanogaster.. Genetics 139:1663-1678[Abstract].

KARPEN, G. H. and A. C. SPRADLING, 1992  Analysis of subtelomeric heterochromatin in a Drosophila minichromosome by single P element insertional mutagenesis. Genetics 132:737-753[Abstract].

KARSCH-MIZRACHI, I. and S. R. HAYNES, 1993  The Rb97D gene encodes a potential RNA-binding protein required for spermatogenesis in Drosophila. Nucleic Acids Res. 21:2229-2235[Abstract/Free Full Text].

KAUFFMANN, R. C., S. LI, P. A. GALLAGHER, J. ZHANG, and R. W. CARTHEW, 1996  Ras1 signaling and transcriptional competence in the R7 cell of Drosophila. Genes Dev. 10:2167-2178[Abstract/Free Full Text].

KELLEY, R. L., 1993  Initial organization of the Drosophila dorsoventral axis depends on an RNA-binding protein encoded by the squid gene. Genes Dev. 7:948-960[Abstract/Free Full Text].

KEYES, L. N. and A. C. SPRADLING, 1997  The Drosophila gene fs(2)cup interacts with otu to define a cytoplasmic pathway required for the structure and function of germ-line chromosomes. Development 124:1419-1431[Abstract].

KIDWELL, M., 1986 P-M mutagenesis, pp. 59–81 in Drosophila: A Practical Approach, edited by D. B. ROBERTS. IRL, Oxford.

KLECKNER, N., J. ROTH, and D. BOTSTEIN, 1977  Genetic engineering in vivo using translocatable drug-resistance elements. New methods in bacterial genetics. J. Mol. Biol. 116:125-159[Medline].

KLOSS, B., J. L. PRICE, L. SAEZ, J. BLAU, and A. ROTHENFLUH et al., 1998  The Drosophila clock gene double-time encodes a protein closely related to human casein kinase Iepsilon. Cell 94:97-107[Medline].

KNOBLICH, J. A., K. SAUER, L. JONES, H. RICHARDSON, and R. SAINT et al., 1994  Cyclin E controls S phase progression and its down-regulation during Drosophila embryogenesis is required for the arrest of cell proliferation. Cell 77:107-120[Medline].

KOCKEL, L., G. VORBRUGGEN, H. JACKLE, M. MLODZIK, and D. BOHMANN, 1997  Requirement for Drosophila 14-3-3 zeta in Raf-dependent photoreceptor development. Genes Dev. 11:1140-1147[Abstract/Free Full Text].

KOLHEKAR, A. S., M. S. ROBERTS, N. JIANG, R. C. JOHNSON, and R. E. MAINS et al., 1997  Neuropeptide amidation in Drosophila: separate genes encode the two enzymes catalyzing amidation. J. Neurosci. 17:1363-1376[Abstract/Free Full Text].

KOLODKIN, A. L., D. J. MATTHES, and C. S. GOODMAN, 1993  The semaphorin genes encode a family of transmembrane and secreted growth cone guidance molecules. Cell 75:1389-1399[Medline].

KORSWAGEN, H. C., R. M. DURBIN, M. T. SMITS, and R. H. PLASTERK, 1996  Transposon Tc1-derived, sequence-tagged sites in Caenorhabditis elegans as markers for gene mapping. Proc. Natl. Acad. Sci. USA 93:14680-14685[Abstract/Free Full Text].

KOZLOVA, T., G. V. POKHOLKOVA, G. TZERTZINIS, J. D. SUTHERLAND, and I. F. ZHIMULEV et al., 1998  Drosophila hormone receptor 38 functions in metamorphosis: a role in adult cuticle formation. Genetics 149:1465-1475[Abstract/Free Full Text].

KUSSEL, P. and M. FRASCH, 1995  Pendulin, a Drosophila protein with cell cycle-dependent nuclear localization, is required for normal cell proliferation. J. Cell Biol. 129:1491-1507[Abstract/Free Full Text].

LANTZ, V., L. AMBROSIO, and P. SCHEDL, 1992  The Drosophila orb gene is predicted to encode sex-specific germline RNA-binding proteins and has localized transcripts in ovaries and early embryos. Development 115:75-88[Abstract].

LEE, J. J., D. VON KESSLER, S. PARKS, and P. A. BEACHY, 1992  Secretion and localized transcription suggest a role in positional signaling for products of the segmentation gene hedgehog.. Cell 71:33-50[Medline].

LEHNER, C. F. and P. H. O'FARRELL, 1989  Expression and function of Drosophila cyclin A during embryonic cell cycle progression. Cell 56:957-968[Medline].

LEKVEN, A. C., U. TEPASS, M. KESHMESHIAN, and V. HARTENSTEIN, 1998  faint sausage encodes a novel extracellular protein of the immunoglobulin superfamily required for cell migration and the establishment of normal axonal pathways in the Drosophila nervous system. Development 125:2747-2758[Abstract].

LEPAGE, T., S. M. COHEN, F. J. DIAZ-BENJUMEA, and S. M. PARKHURST, 1995  Signal transduction by cAMP-dependent protein kinase A in Drosophila limb patterning. Nature 373:711-715[Medline].

LETSOU, A., K. ARORA, J. L. WRANA, K. SIMIN, and V. TWOMBLY et al., 1995  Drosophila Dpp signaling is mediated by the punt gene product: a dual ligand-binding type II receptor of the TGF beta receptor family. Cell 80:899-908[Medline].

LEVINE, A., A. BASHAN-AHREND, O. BUDAI-HADRIAN, D. GARTENBERG, and S. MENASHEROW et al., 1994  Odd Oz: a novel Drosophila pair rule gene. Cell 77:587-598[Medline].

LIN, H. and A. C. SPRADLING, 1993  Germline stem cell division and egg chamber development in transplanted Drosophila germaria. Dev. Biol. 159:140-152[Medline].

LIN, H. and A. C. SPRADLING, 1997  A novel group of pumilio mutations affects the asymmetric division of germline stem cells in the Drosophila ovary. Development 124:2463-2476[Abstract].

LIN, W. H., L. H. HUANG, J. Y. YEH, J. HOHEISEL, and H. LEHRACH et al., 1995  Expression of a Drosophila GATA transcription factor in multiple tissues in the developing embryos: identification of homozygous lethal mutants with P-element insertion at the promoter region. J. Biol. Chem. 270:25150-25158[Abstract/Free Full Text].

LO, P. C. H. and M. FRASCH, 1998  bagpipe-dependent expression of vimar, a novel armadillo-repeats gene, in Drosophila visceral mesoderm. Mech. Dev. 72:65-75[Medline].

MANCEBO, R., P. C. LO, and S. M. MOUNT, 1990  Structure and expression of the Drosophila melanogaster gene for the U1 small nuclear ribonucleoprotein particle 70K protein. Mol. Cell. Biol. 10:2492-2502[Abstract/Free Full Text].

MARDON, G., N. M. SOLOMON, and G. M. RUBIN, 1994  dachshund encodes a nuclear protein required for normal eye and leg development in Drosophila. Development 120:3473-3486[Abstract].

MARTIN-BLANCO, E. and A. A. GARCIA-BELLIDO, 1996  Mutations in the rotated abdomen locus affect muscle development and reveal an intrinsic asymmetry in Drosophila. Proc. Natl. Acad. Sci. USA 93:6048-6052[Abstract/Free Full Text].

MATHIES, L. D., S. KERRIDGE, and M. P. SCOTT, 1994  Role of the teashirt gene in Drosophila midgut morphogenesis: secreted proteins mediate the action of homeotic genes. Development 120:2799-2809[Abstract].

MEINKE, D. W., J. M. CHERRY, C. DEAN, S. D. ROUNSLEY, and M. KOORNNEEF, 1998  Arabidopsis thaliana: a model plant for genome analysis. Science 282:662-682[Abstract/Free Full Text].

MELLERICK, D. M., J. A. KASSIS, S. D. ZHANG, and W. F. ODENWALD, 1992  Castor encodes a novel zinc finger protein required for the development of a subset of CNS neurons in Drosophila. Neuron 9:789-803[Medline].

MCKEARIN, D. and A. C. SPRADLING, 1990  Bag-of-marbles: a Drosophila gene required to initiate both male and female gametogenesis. Genes Dev. 4:2242-2251[Abstract/Free Full Text].

MCKIM, K. S. and A. HAYASHI-HAGIHARA, 1998  mei-W68 in Drosophila melanogaster encodes a Spo11 homolog: evidence that the mechanism for initiating meiotic recombination is conserved. Genes Dev. 12:2932-2942[Abstract/Free Full Text].

MIKLOS, G. L. and G. M. RUBIN, 1996  The role of the genome project in determining gene function: insights from model organisms. Cell 86:521-529[Medline].

MLODZIK, M., Y. HIROMI, U. WEBER, C. S. GOODMAN, and G. M. RUBIN, 1990  The Drosophila seven-up gene, a member of the steroid receptor gene superfamily, controls photoreceptor cell fates. Cell 60:211-224[Medline].

MOHLER, J., J. W. MAHAFFEY, E. DEUTSCH, and K. VANI, 1995  Control of Drosophila head segment identity by the bZIP homeotic gene cnc. Development 121:237-247[Abstract].

MONTELL, D. J., P. RØRTH, and A. C. SPRADLING, 1992  slow border cells, a locus required for a developmentally regulated cell migration during oogenesis, encodes Drosophila C/EBP. Cell 71:51-62[Medline].

MURPHY, A. M., T. LEE, C. M. ANDREWS, B. Z. SHILO, and D. J. MONTELL, 1995  The breathless FGF receptor homolog, a downstream target of Drosophila C/EBP in the developmental control of cell migration. Development 121:2255-2263[Abstract].

NAKATO, H., T. A. FUTCH, and S. B. SELLECK, 1995  The division abnormally delayed, dally, gene: a putative integral membrane proteoglycan required for cell division patterning during postembryonic development of the nervous system in Drosophila. Development 121:3687-3702[Abstract].

NEUFELD, T. P. and G. M. RUBIN, 1994  The Drosophila peanut gene is required for cytokinesis and encodes a protein similar to yeast putative bud neck filament proteins. Cell 77:371-379[Medline].

NEUFELD, T. P., A. H. TANG, and G. M. RUBIN, 1998  A genetic screen to identify components of the sina signaling pathway in Drosophila eye development. Genetics 148:277-286[Abstract/Free Full Text].

NIBU, Y., H. ZHANG, and M. LEVINE, 1998  Interaction of short-range repressors with Drosophila CtBP in the embryo. Science 280:101-104[Abstract/Free Full Text].

NOZAKI, M., Y. ONISHI, S. TOGASHI, and H. MIYAMOTO, 1996  Molecular characterization of the Drosophila Mo25 gene, which is conserved among Drosophila, mouse, and yeast. DNA Cell Biol. 15:505-509[Medline].

OKANO, H., S. HAYASHI, T. TANIMURA, K. SAWAMOTO, and S. YOSHIKAWA et al., 1992  Regulation of Drosophila neural development by a putative secreted protein. Differentiation 52:1-11[Medline].

O'NEILL, E. M., I. REBAY, R. TJIAN, and G. M. RUBIN, 1994  The activities of two Ets-related transcription factors required for Drosophila eye development are modulated by the Ras/MAPK pathway. Cell 78:137-147[Medline].

PARK, M., X. WU, K. GOLDEN, J. D. AXELROD, and R. BODMER, 1996  The wingless signaling pathway is directly involved in Drosophila heart development. Dev. Biol. 177:104-116[Medline].

PERRIMON, N., A. LANJUIN, C. ARNOLD, and E. NOLL, 1996  Zygotic lethal mutations with maternal effect phenotypes in Drosophila melanogaster. Part II. Loci on the second and third chromosomes identified by P-element-induced mutations. Genetics 144:1681-1692[Abstract].

PETERSEN, S. A., R. D. FETTER, J. N. NOORDERMEER, C. S. GOODMAN, and A. DIANTONIO, 1997  Genetic analysis of glutamate receptors in Drosophila reveals a retrograde signal regulating presynaptic transmitter release. Neuron 19:1237-1248[Medline].

PLASTERK, R. H., 1993  Reverse genetics of Caenorhabditis elegans.. Bioessays 14:629-633.

RAUSKOLB, C., K. M. SMITH, M. PEIFER, and E. WIESCHAUS, 1995  Extradenticle determines segmental identities throughout Drosophila development. Development 121:3663-3673[Abstract].

REHORN, K. P., H. THELEN, A. M. MICHELSON, and R. REUTER, 1996  A molecular aspect of hematopoiesis and endoderm development common to vertebrates and Drosophila. Development 122:4023-4031[Abstract].

RIECKHOF, G. E., F. CASARES, H. D. RYOO, M. ABU-SHAAR, and R. S. MANN, 1997  Nuclear translocation of extradenticle requires homothorax, which encodes an extradenticle-related homeodomain protein. Cell 91:171-183[Medline].

RITTENHOUSE, K. R. and C. A. BERG, 1995  Mutations in the Drosophila gene bullwinkle cause the formation of abnormal eggshell structures and bicaudal embryos. Development 121:3023-3033[Abstract].

ROCH, F., F. SERRAS, F. J. CIFUENTES, M. COROMINAS, and B. ALSINA et al., 1998  Screening of larval/pupal P-element induced lethals on the second chromosome in Drosophila melanogaster: clonal analysis and morphology of imaginal discs. Mol. Gen. Genet. 257:103-112[Medline].

RODRIGUEZ, A., Z. ZHOU, M. L. TANG, S. MELLER, and J. CHEN et al., 1996  Identification of immune system and response genes, and novel mutations causing melanotic tumor formation in Drosophila melanogaster. Genetics 143:929-940[Abstract].

ROOKE, J., D. PAN, T. XU, and G. M. RUBIN, 1996  KUZ, a conserved metalloprotease-disintegrin protein with two roles in Drosophila neurogenesis. Science 273:1227-1231[Abstract].

RØRTH, P., 1996  A modular misexpression screen in Drosophila detecting tissue-specific phenotypes. Proc. Natl. Acad. Sci. USA 93:12418-12422[Abstract/Free Full Text].

RØRTH, P., K. SZABO, A. BAILEY, T. LAVERTY, and J. REHM et al., 1998  Systematic gain-of-function genetics in Drosophila. Development 125:1049-1057[Abstract].

ROTTGEN, G., T. WAGNER, and G. HINZ, 1998  A genetic screen for elements of the network that regulates neurogenesis in Drosophila. Mol. Gen. Genet. 257:442-451[Medline].

ROULIER, E. M., S. PANZER, and S. K. BECKENDORF, 1998  The Tec29 tyrosine kinase is required during Drosophila embryogenesis and interacts with Src64 in ring canal development. Mol. Cell 6:819-829.

RUBERTE, E., T. MARTY, D. NELLEN, M. AFFOLTER, and K. BASLER, 1995  An absolute requirement for both the Type II and Type I receptors, punt and thick veins, for Dpp signaling in vivo. Cell 80:889-897[Medline].

RUDEN, D. M., W. CUI, V. SOLLARS, and M. A. ALTERMAN, 1997  Drosophila kinesin-like protein (Klp38B) functions during meiosis, mitosis, and segmentation. Dev. Biol. 191:284-296[Medline].

RUDNER, D. Z., R. KANAAR, K. S. BREGER, and D. C. RIO, 1996  Mutations in the small subunit of the Drosophila U2AF splicing factor cause lethality and developmental defects. Proc. Natl. Acad. Sci. USA 93:10333-10337[Abstract/Free Full Text].

RUSSELL, S. R. H., G. HEIMBECK, C. M. GODDARD, A. T. C. CARPENTER, and M. ASHBURNER, 1996  The Drosophila Eip78C gene is not vital but has a role in regulating chromosome puffs. Genetics 144:159-170[Abstract].

RUSSELL, M. A., L. OSTAFICHUK, and S. SCANGA, 1998  Lethal P-lacZ insertion lines expressed during pattern respecification in the imaginal discs of Drosophila. Genome 41:7-13[Medline].

SALZBERG, A., K. GOLDEN, R. BODMER, and H. J. BELLEN, 1996  gutfeeling, a Drosophila gene encoding an antizyme-like protein, is required for late differentiation of neurons and muscles. Genetics 144:183-196[Abstract].

SAMAKOVLIS, C., G. MANNING, P. STENEBERG, N. HACOHEN, and R. CANTERA et al., 1996  Genetic control of epithelial tube fusion during Drosophila tracheal development. Development 122:3531-3536[Abstract].

SAVANT-BHONSALE, S. and D. J. MONTELL, 1993  Torso-like encodes the localized determinant of Drosophila terminal pattern formation. Genes Dev. 7:2548-2555[Abstract/Free Full Text].

SCHMUCKER, D., H. JACKLE, and U. GAUL, 1997  Genetic analysis of the larval optic nerve projection in Drosophila. Development 124:937-948[Abstract].

SCHNEIDER, L. E. and A. C. SPRADLING, 1997  The Drosophila G-protein-coupled receptor kinase homologue Gprk2 is required for egg morphogenesis. Development 124:2591-2602[Abstract].

SCHNORR, J. D. and C. A. BERG, 1996  Differential activity of Ras1 during patterning of the Drosophila dorsoventral axis. Genetics 144:1545-1557[Abstract].

SCHULZE, K. L., K. BROADIE, M. S. PERIN, and H. J. BELLEN, 1995  Genetic and electrophysiological studies of Drosophila Syntaxin-1A demonstrate its role in nonneuronal secretion and neurotransmission. Cell 80:311-320[Medline].

SIEGEL, V., T. A. JONGENS, L. Y. JAN, and Y. N. JAN, 1993  pipsqueak, an early acting member of the posterior group of genes, affects vasa level and germ cell-somatic cell interaction in the developing egg chamber. Development 119:1187-1202[Abstract].

SIMON, M. A., G. S. DODSON, and G. M. RUBIN, 1993  An SH3-SH2-SH3 protein is required for p21Ras1 activation and binds to sevenless and Sos proteins in vitro. Cell 73:169-177[Medline].

SISSON, J. C., K. S. HO, K. SUYAMA, and M. P. SCOTT, 1997  Costal2, a novel kinesin-related protein in the Hedgehog signaling pathway. Cell 90:235-245[Medline].

SLITER, T. J., V. C. HENRICH, R. L. TUCKER, and L. I. GILBERT, 1989  The genetics of the Dras3-Roughened-ecdysoneless chromosomal region (62B3-4 to 62D3-4) in Drosophila melanogaster: analysis of recessive lethal mutations. Genetics 123:327-336[Abstract/Free Full Text].

SMITH, D., Y. YANAI, Y. G. LIE, S. ISHIGURO, and K. OKADA et al., 1996  Characterization and mapping of Ds-GUS-T-DNA lines for targeted insertional mutagenesis. Plant J. 10:721-732[Medline].

SONG, Z., K. MCCALL, and H. STELLER, 1997  DCP-1, a Drosophila cell death protease essential for development. Science 275:536-540[Abstract/Free Full Text].

SOTILLOS, S., F. ROCH, and S. CAMPUZANO, 1997  The metalloprotease-disintegrin Kuzbanian participates in Notch activation during growth and patterning of Drosophila imaginal discs. Development 124:4769-4779[Abstract].

SOZEN, M. A., J. D. ARMSTRONG, M. YANG, K. KAISER, and J. A. T. DOW, 1997  Functional domains are specified to single-cell resolution in a Drosophila epithelium. Proc. Natl. Acad. Sci. USA 94:5207-5212[Abstract/Free Full Text].

SPRADLING, A. C., D. M. STERN, I. KISS, J. FOOTE, and T. LAVERTY et al., 1995  Gene disruptions using P transposable elements: an integral component of the Drosophila genome project. Proc. Natl. Acad. Sci. USA 92:10824-10830[Abstract/Free Full Text].

STARK, K. A., G. H. YEE, C. E. ROOTE, E. L. WILLIAMS, and S. ZUSMAN et al., 1997  A novel alpha integrin subunit associates with betaPS and functions in tissue morphogenesis and movement during Drosophila development. Development 124:4583-4594[Abstract].

STELLER, H. and V. PIRROTTA, 1986  P transposons controlled by the heat shock promoter. Mol. Cell. Biol. 6:1640-1649[Abstract/Free Full Text].

STROUMBAKIS, N. D., Z. LI, and P. P. TOLIAS, 1996  A homolog of human transcription factor NF-X1 encoded by the Drosophila shuttle craft gene is required in the embryonic central nervous system. Mol. Cell. Biol. 16:192-201[Abstract].

STRUTT, D. I., U. WEBER, and M. MLODZIK, 1997  The role of RhoA in tissue polarity and Frizzled signalling. Nature 387:292-295[Medline].

SULLIVAN, W., P. FOGARTY, and W. E. THEURKAUF, 1993  Mutations affecting the cytoskeletal organization of syncytial Drosophila embryos. Development 118:1245-1254[Abstract].

SUNDARESAN, V., P. SPRINGER, T. VOLPE, S. HAWARD, J. D. G. JONES, C. DEAN, H. MA, and R. MARTIENSSEN, 1995  Patterns of gene action in plant development revealed by enhancer trap and gene trap transposable elements. Genes Dev. 9:1797-1810[Abstract/Free Full Text].

TAYLOR, C. A., K. N. STANLEY, and A. D. SHIRRAS, 1997  The Orct gene of Drosophila melanogaster codes for a putative organic cation transporter with six or 12 transmembrane domains. Gene 201:69-74[Medline].

TEPASS, U., E. GRUSZYNSKI-DEFEO, T. A. HAAG, L. OMATYAR, and T. TOROK et al., 1996  shotgun encodes Drosophila E-cadherin and is preferentially required during cell rearrangement in the neurectoderm and other morphogenetically active epithelia. Genes Dev. 10:672-685[Abstract/Free Full Text].

TETZLAFF, M. T., H. JAECKLE, and M. J. PANKRATZ, 1996  Lack of Drosophila cytoskeletal tropomyosin effects head morphogenesis and the accumulation of oskar mRNA required to germ cell formation. EMBO J. 15:1247-1254[Medline].

THERRIEN, M., H. C. Y. CHANG, N. M. SOLOMON, F. D. KARIM, and D. A. WASSARMAN et al., 1995  KSR, a novel protein kinase required for RAS signal transduction. Cell 83:879-888[Medline].

THERRIEN, M., A. M. WONG, and G. M. RUBIN, 1998  CNK, a FAF-binding multidomain protein required for RAS signaling. Cell 95:343-353[Medline].

TÖROK, T., T. TICK, M. ALVARADO, and I. KISS, 1993  P-lacW insertional mutagenesis on the second chromosome of Drosophila melanogaster: isolation of lethals with different overgrowth phenotypes. Genetics 135:71-80[Abstract].

TÖROK, T., P. D. HARVIE, M. BURATOVICH, and P. J. BRYANT, 1997  The product of proliferation disrupter is concentrated at centromeres and required for mitotic chromosome condensation and cell proliferation in Drosophila. Genes Dev. 11:213-225[Abstract/Free Full Text].

TREISMAN, J. E. and G. M. RUBIN, 1996  Targets of glass regulation in the Drosophila eye disc. Mech. Dev. 56:17-24[Medline].

TREISMAN, J. E., P. J. FOLLETTE, P. H. O'FARRELL, and G. M. RUBIN, 1995a  Cell proliferation and DNA replication defects in a Drosophila MCM2 mutant. Genes Dev. 9:1709-1715[Abstract/Free Full Text].

TREISMAN, J. E., Z. C. LAI, and G. M. RUBIN, 1995b  Shortsighted acts in the decapentaplegic pathway in Drosophila eye development and has homology to a mouse TGF-beta-responsive gene. Development 121:2835-2845[Abstract].

TREISMAN, J. E., N. ITO, and G. M. RUBIN, 1997a  misshapen encodes a protein kinase involved in cell shape control in Drosophila. Gene 186:119-125[Medline].

TREISMAN, J. E., A. LUK, G. M. RUBIN, and U. HEBERLEIN, 1997b  eyelid antagonizes wingless signaling during Drosophila development and has homology to the Bright family of DNA-binding proteins. Genes Dev. 11:1949-1962[Abstract/Free Full Text].

TSUNEIZUMI, K., T. NAKAYAMA, Y. KAMOSHIDA, T. B. KORNBERG, and J. L. CHRISTIAN et al., 1997  Daughters against dpp modulates dpp organizing activity in Drosophila wing development. Nature 389:627-631[Medline].

TWOMBLY, V., R. K. BLACKMAN, H. JIN, J. M. GRAFF, and R. W. PADGETT et al., 1996  The TGF-beta signaling pathway is essential for Drosophila oogenesis. Development 122:1555-1565[Abstract].

UEMURA, T., S. SHEPHERD, L. ACKERMAN, L. Y. JAN, and Y. N. JAN, 1989  numb, a gene required in determination of cell fate during sensory organ formation in Drosophila embryos. Cell 58:349-360[Medline].

UEMURA, T., K. SHIOMI, S. TOGASHI, and M. TAKEICHI, 1993  Mutation of twins encoding a regulator of protein Phosphatase 2A leads to pattern duplication in Drosophila imaginal discs. Genes Dev. 7:429-440[Abstract/Free Full Text].

UEMURA, T., H. ODA, R. KRAUT, S. HAYASHI, Y. KOTAOKA, and M. TAKEICHI, 1996  Zygotic Drosophila E-cadherin expression is required for processes of dynamic epithelial cell rearrangements in the Drosophila embryo. Genes Dev. 10:659-671[Abstract/Free Full Text].

VAN DER STRATEN, A., C. ROMMEL, B. DICKSON, and E. HAFEN, 1997  The heat shock protein 83 (Hsp83) is required for Raf-mediated signalling in Drosophila. EMBO J. 16:1961-1969[Medline].

VANKATESH, K. and G. HASAN, 1997  Disruption of the IP3 receptor gene of Drosophila affects larval metamorphosis and ecdysone release. Curr. Biol. 7:500-509[Medline].

VENTER, J. C., M. D. ADAMS, G. G. SUTTON, A. R. KERLAVAGE, and H. O. SMITH et al., 1998  Shotgun sequencing of the human genome. Science 280:1540-1542[Free Full Text].

VERHEYEN, E. M., K. J. PURCELL, M. E. FORTINI, and S. ARTAVANIS-TSAKONAS, 1996  Analysis of dominant enhancers and suppressors of activated Notch in Drosophila. Genetics 144:1127-1141[Abstract].

WASSARMAN, D. A., N. M. SOLOMON, H. C. Y. CHANG, F. D. KARIM, and M. THERRIEN et al., 1996  Protein phosphatase 2A positively and negatively regulates Ras1-mediated photoreceptor development in Drosophila. Genes Dev. 10:272-278[Abstract/Free Full Text].

WILK, R., I. WEIZMAN, and B. Z. SHILO, 1996  trachealess encodes a bHLH-PAS protein that is an inducer of tracheal cell fates in Drosophila. Genes Dev. 10:93-102[Abstract/Free Full Text].

WURST, W., J. ROSSANT, V. PRIDEAUX, M. KOWNACKA, and A. JOYNER et al., 1995  A large-scale gene-trap screen for insertional mutations in developmentally regulated genes in mice. Genetics 139:889-899[Abstract].

XIONG, W. C. and C. MONTELL, 1993  tramtrack is a transcriptional repressor required for cell fate determination in the Drosophila eye. Genes Dev. 7:1085-1096[Abstract/Free Full Text].

XIONG, W. C., H. OKANO, N. H. PATEL, J. A. BLENDY, and C. MONTELL, 1994  Repo encodes a glial-specific homeo domain protein required in the Drosophila nervous system. Genes Dev. 8:981-994[Abstract/Free Full Text].

XUE, F. and L. COOLEY, 1993  kelch encodes a component of intercellular bridges in Drosophila egg chambers. Cell 72:681-693[Medline].

YANG, X., S. BAHRI, T. KLEIN, and W. CHIA, 1997  Klumpfuss, a putative Drosophila zinc finger transcription factor, acts to differentiate between the identities of two secondary precursor cells within one neuroblast lineage. Genes Dev. 11:1396-1408[Abstract/Free Full Text].

YARNITZKY, T., L. MIN, and T. VOLK, 1997  The Drosophila neuregulin homolog vein mediates inductive interactions between myotubes and their epidermal attachment cells. Genes Dev. 11:2691-2700[Abstract/Free Full Text].

YASOTHORNSRIKUL, S., W. J. DAVIS, G. CRAMER, D. A. KIMBRELL, and C. R. DEAROLF, 1997  viking: dentification and characterization of a second type IV collagen in Drosophila. Gene 198:17-25[Medline].

YU, Y., W. LI, K. SU, M. YUSSA, and W. HAN et al., 1997  The nuclear hormone receptor Ftz-F1 is a cofactor for the Drosophila homeodomain protein Ftz. Nature 385:552-555[Medline].

YU, H. H., H. H. ARAJ, S. A. RALLS, and A. L. KOLODKIN, 1998  The transmembrane Semaphorin Sema I is required in Drosophila for embryonic motor and CNS axon guidance. Neuron 20:207-220[Medline].

YUE, L. and A. C. SPRADLING, 1992  hu-li tai shao, a gene required for ring canal formation during Drosophila oogenesis, encodes a homolog of adducin. Genes Dev. 6:2443-2454[Abstract/Free Full Text].

ZAMBROWICZ, B. P., G. A. FRIEDRICH, E. C. BUXTON, S. L. LILLEBERG, and C. PERSON et al., 1998  Disruption and sequence identification of 2,000 genes in mouse embryonic stem cells. Nature 392:608-611[Medline].

ZHANG, P. and A. C. SPRADLING, 1995  The Drosophila salivary gland chromocenter contains highly polytenized subdomains of mitotic heterochromatin. Genetics 139:659-670[Abstract].

ZHANG, N., J. ZHANG, K. J. PURCELL, Y. CHENG, and K. HOWARD, 1997  The Drosophila protein Wunen repels migrating germ cells. Nature 385:64-67[Medline].

ZHANG, B., Y. H. KOH, R. B. BECKSTEAD, V. BUDNIK, and B. GANETZKY et al., 1998  Synaptic vesicle size and number are regulated by a clathrin adaptor protein required for endocytosis. Neuron 21:1465-1475[Medline].

ZHOU, Q. and D. S. HAYMER, 1997  Molecular structure of yoyo, a gypsy-like retrotransposon from the mediterranean fruit fly, Ceratitis capitata.. Genetica 101:167-178[Medline].

ZUR LAGE, P., A. D. SHRIMPTON, A. J. FLAVELL, T. F. MACKAY, and A. J. BROWN, 1997  Genetic and molecular analysis of smooth, a quantitative trait locus affecting bristle number in Drosophila melanogaster.. Genetics 146:607-618[Abstract].

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				E. A. Sevrioukov, N. Moghrabi, M. Kuhn, and H. Kramer A Mutation in dVps28 Reveals a Link between a Subunit of the Endosomal Sorting Complex Required for Transport-I Complex and the Actin Cytoskeleton in Drosophila Mol. Biol. Cell, May 1, 2005; 16(5): 2301 - 2312. [Abstract] [Full Text] [PDF]

				S. Srinivasan, J. A. Armstrong, R. Deuring, I. K. Dahlsveen, H. McNeill, and J. W. Tamkun The Drosophila trithorax group protein Kismet facilitates an early step in transcriptional elongation by RNA Polymerase II Development, April 1, 2005; 132(7): 1623 - 1635. [Abstract] [Full Text] [PDF]

				M. R. MacPherson, V. P. Pollock, L. Kean, T. D. Southall, M. E. Giannakou, K. E. Broderick, J. A. T. Dow, R. C. Hardie, and S. A. Davies Transient Receptor Potential-Like Channels Are Essential for Calcium Signaling and Fluid Transport in a Drosophila Epithelium Genetics, March 1, 2005; 169(3): 1541 - 1552. [Abstract] [Full Text] [PDF]

				L. Ferrarini, L. Bertelli, J. Feala, A. D. McCulloch, and G. Paternostro A more efficient search strategy for aging genes based on connectivity Bioinformatics, February 1, 2005; 21(3): 338 - 348. [Abstract] [Full Text] [PDF]

				B. T. Sage, J. L. Jones, A. L. Holmes, M. D. Wu, and A. K. Csink Sequence Elements in cis Influence Heterochromatic Silencing in trans Mol. Cell. Biol., January 1, 2005; 25(1): 377 - 388. [Abstract] [Full Text] [PDF]

				G. A. Shanower, M. Muller, J. L. Blanton, V. Honti, H. Gyurkovics, and P. Schedl Characterization of the grappa Gene, the Drosophila Histone H3 Lysine 79 Methyltransferase Genetics, January 1, 2005; 169(1): 173 - 184. [Abstract] [Full Text] [PDF]

				H. K. Salz, R. S. Y. Mancebo, A. A. Nagengast, O. Speck, M. Psotka, and S. M. Mount The Drosophila U1-70K Protein Is Required for Viability, but Its Arginine-Rich Domain Is Dispensable Genetics, December 1, 2004; 168(4): 2059 - 2065. [Abstract] [Full Text] [PDF]

				I. Miguel-Aliaga, D. W. Allan, and S. Thor Independent roles of the dachshund and eyes absent genes in BMP signaling, axon pathfinding and neuronal specification Development, December 1, 2004; 131(23): 5837 - 5848. [Abstract] [Full Text] [PDF]

				A. I. Ivanov, A. C. Rovescalli, P. Pozzi, S. Yoo, B. Mozer, H.-P. Li, S.-H. Yu, H. Higashida, V. Guo, M. Spencer, et al. Genes required for Drosophila nervous system development identified by RNA interference PNAS, November 16, 2004; 101(46): 16216 - 16221. [Abstract] [Full Text] [PDF]

				J. W. Park, K. Parisky, A. M. Celotto, R. A. Reenan, and B. R. Graveley From the Cover: Identification of alternative splicing regulators by RNA interference in Drosophila PNAS, November 9, 2004; 101(45): 15974 - 15979. [Abstract] [Full Text] [PDF]

				K. Kato, T. Chihara, and S. Hayashi Hedgehog and Decapentaplegic instruct polarized growth of cell extensions in the Drosophila trachea Development, November 1, 2004; 131(21): 5253 - 5261. [Abstract] [Full Text] [PDF]

				H. Qi, U. Rath, D. Wang, Y.-Z. Xu, Y. Ding, W. Zhang, M. J. Blacketer, M. R. Paddy, J. Girton, J. Johansen, et al. Megator, an Essential Coiled-Coil Protein that Localizes to the Putative Spindle Matrix during Mitosis in Drosophila Mol. Biol. Cell, November 1, 2004; 15(11): 4854 - 4865. [Abstract] [Full Text] [PDF]

				M. W. Kankel, D. M. Duncan, and I. Duncan A Screen for Genes That Interact With the Drosophila Pair-Rule Segmentation Gene fushi tarazu Genetics, September 1, 2004; 168(1): 161 - 180. [Abstract] [Full Text] [PDF]

				D. D. Pollock and J. C. Larkin Estimating the Degree of Saturation in Mutant Screens Genetics, September 1, 2004; 168(1): 489 - 502. [Abstract] [Full Text] [PDF]

				A. J. Moehring and T. F. C. Mackay The Quantitative Genetic Basis of Male Mating Behavior in Drosophila melanogaster Genetics, July 1, 2004; 167(3): 1249 - 1263. [Abstract] [Full Text] [PDF]

				A. Pavlopoulos, A. J. Berghammer, M. Averof, and M. Klingler Efficient Transformation of the Beetle Tribolium castaneum Using the Minos Transposable Element: Quantitative and Qualitative Analysis of Genomic Integration Events Genetics, June 1, 2004; 167(2): 737 - 746. [Abstract] [Full Text] [PDF]

				H. J. Bellen, R. W. Levis, G. Liao, Y. He, J. W. Carlson, G. Tsang, M. Evans-Holm, P. R. Hiesinger, K. L. Schulze, G. M. Rubin, et al. The BDGP Gene Disruption Project: Single Transposon Insertions Associated With 40% of Drosophila Genes Genetics, June 1, 2004; 167(2): 761 - 781. [Abstract] [Full Text] [PDF]

				A. Ghosh-Roy, M. Kulkarni, V. Kumar, S. Shirolikar, and K. Ray Cytoplasmic Dynein-Dynactin Complex Is Required for Spermatid Growth but Not Axoneme Assembly in Drosophila Mol. Biol. Cell, May 1, 2004; 15(5): 2470 - 2483. [Abstract] [Full Text] [PDF]

				S. Urban, G. Brown, and M. Freeman EGF receptor signalling protects smooth-cuticle cells from apoptosis during Drosophila ventral epidermis development Development, April 15, 2004; 131(8): 1835 - 1845. [Abstract] [Full Text] [PDF]

				A. C. Groth, M. Fish, R. Nusse, and M. P. Calos Construction of Transgenic Drosophila by Using the Site-Specific Integrase From Phage {phi}C31 Genetics, April 1, 2004; 166(4): 1775 - 1782. [Abstract] [Full Text] [PDF]

				E. S. Montana and J. T. Littleton Characterization of a hypercontraction-induced myopathy in Drosophila caused by mutations in Mhc J. Cell Biol., March 29, 2004; 164(7): 1045 - 1054. [Abstract] [Full Text] [PDF]

				H. C. Chang, M. Hull, and I. Mellman The J-domain protein Rme-8 interacts with Hsc70 to control clathrin-dependent endocytosis in Drosophila J. Cell Biol., March 29, 2004; 164(7): 1055 - 1064. [Abstract] [Full Text] [PDF]

				H. H. Kazazian Jr. Mobile Elements: Drivers of Genome Evolution Science, March 12, 2004; 303(5664): 1626 - 1632. [Abstract] [Full Text] [PDF]

				S. H. Myster, F. Wang, R. Cavallo, W. Christian, S. Bhotika, C. T. Anderson, and M. Peifer Genetic and Bioinformatic Analysis of 41C and the 2R Heterochromatin of Drosophila melanogaster: A Window on the Heterochromatin-Euchromatin Junction Genetics, February 1, 2004; 166(2): 807 - 822. [Abstract] [Full Text] [PDF]

				K. Patterson, A. B. Molofsky, C. Robinson, S. Acosta, C. Cater, and J. A. Fischer The Functions of Klarsicht and Nuclear Lamin in Developmentally Regulated Nuclear Migrations of Photoreceptor Cells in the Drosophila Eye Mol. Biol. Cell, February 1, 2004; 15(2): 600 - 610. [Abstract] [Full Text] [PDF]

				R. J. Kelso, M. Buszczak, A. T. Quinones, C. Castiblanco, S. Mazzalupo, and L. Cooley Flytrap, a database documenting a GFP protein-trap insertion screen in Drosophila melanogaster Nucleic Acids Res., January 1, 2004; 32(90001): D418 - 420. [Abstract] [Full Text] [PDF]

				J. Gates, G. Lam, J. A. Ortiz, R. Losson, and C. S. Thummel rigor mortis encodes a novel nuclear receptor interacting protein required for ecdysone signaling during Drosophila larval development Development, January 1, 2004; 131(1): 25 - 36. [Abstract] [Full Text] [PDF]

				C. Estella, G. Rieckhof, M. Calleja, and G. Morata The role of buttonhead and Sp1 in the development of the ventral imaginal discs of Drosophila Development, December 15, 2003; 130(24): 5929 - 5941. [Abstract] [Full Text] [PDF]

				D.-k. Lee, J. W. Park, Y.-J. Kim, J. Kim, Y. Lee, J. Kim, and J.-S. Kim Toward a Functional Annotation of the Human Genome Using Artificial Transcription Factors Genome Res., December 1, 2003; 13(12): 2708 - 2716. [Abstract] [Full Text] [PDF]

				B. Laundrie, J. S. Peterson, J. S. Baum, J. C. Chang, D. Fileppo, S. R. Thompson, and K. McCall Germline Cell Death Is Inhibited by P-Element Insertions Disrupting the dcp-1/pita Nested Gene Pair in Drosophila Genetics, December 1, 2003; 165(4): 1881 - 1888. [Abstract] [Full Text] [PDF]

				T. K. Smulders-Srinivasan and H. Lin Screens for piwi Suppressors in Drosophila Identify Dosage-Dependent Regulators of Germline Stem Cell Division Genetics, December 1, 2003; 165(4): 1971 - 1991. [Abstract] [Full Text] [PDF]

				L. A. Wrischnik, J. R. Timmer, L. A. Megna, and T. W. Cline Recruitment of the Proneural Gene scute to the Drosophila Sex-Determination Pathway Genetics, December 1, 2003; 165(4): 2007 - 2027. [Abstract] [Full Text] [PDF]

				A. Y. Konev, C. M. Yan, D. Acevedo, C. Kennedy, E. Ward, A. Lim, S. Tickoo, and G. H. Karpen Genetics of P-Element Transposition Into Drosophila melanogaster Centric Heterochromatin Genetics, December 1, 2003; 165(4): 2039 - 2053. [Abstract] [Full Text] [PDF]

				J. A. Fraser, P. Kansagra, C. Kotecki, R. D. C. Saunders, and L. I. McLellan The Modifier Subunit of Drosophila Glutamate-Cysteine Ligase Regulates Catalytic Activity by Covalent and Noncovalent Interactions and Influences Glutathione Homeostasis in Vivo J. Biol. Chem., November 21, 2003; 278(47): 46369 - 46377. [Abstract] [Full Text] [PDF]

				V. Dammai, B. Adryan, K. R. Lavenburg, and T. Hsu Drosophila awd, the homolog of human nm23, regulates FGF receptor levels and functions synergistically with shi/dynamin during tracheal development Genes & Dev., November 15, 2003; 17(22): 2812 - 2824. [Abstract] [Full Text] [PDF]

				J. Serano and G. M. Rubin The Drosophila synaptotagmin-like protein bitesize is required for growth and has mRNA localization sequences within its open reading frame PNAS, November 11, 2003; 100(23): 13368 - 13373. [Abstract] [Full Text] [PDF]

				J. M. Shulman and M. B. Feany Genetic Modifiers of Tauopathy in Drosophila Genetics, November 1, 2003; 165(3): 1233 - 1242. [Abstract] [Full Text] [PDF]

				P. J. Clyne, J. S. Brotman, S. T. Sweeney, and G. Davis Green Fluorescent Protein Tagging Drosophila Proteins at Their Native Genomic Loci With Small P Elements Genetics, November 1, 2003; 165(3): 1433 - 1441. [Abstract] [Full Text] [PDF]

				P. Deak, M. Donaldson, and D. M. Glover Mutations in makos, a Drosophila gene encoding the Cdc27 subunit of the anaphase promoting complex, enhance centrosomal defects in polo and are suppressed by mutations in twins/aar, which encodes a regulatory subunit of PP2A J. Cell Sci., October 15, 2003; 116(20): 4147 - 4158. [Abstract] [Full Text] [PDF]

				D. R. Dorer, J. A. Rudnick, E. N. Moriyama, and A. C. Christensen A Family of Genes Clustered at the Triplo-lethal Locus of Drosophila melanogaster Has an Unusual Evolutionary History and Significant Synteny With Anopheles gambiae Genetics, October 1, 2003; 165(2): 613 - 621. [Abstract] [Full Text] [PDF]