A universal method for automated gene mapping
- Peder Zipperlen†1Email author,
- Knud Nairz†2Email author,
- Ivo Rimann2,
- Konrad Basler1,
- Ernst Hafen2,
- Michael Hengartner1 and
- Alex Hajnal2
© Zipperlen et al.; licensee BioMed Central Ltd. 2005
Received: 9 September 2004
Accepted: 9 December 2004
Published: 17 January 2005
Small insertions or deletions (InDels) constitute a ubiquituous class of sequence polymorphisms found in eukaryotic genomes. Here, we present an automated high-throughput genotyping method that relies on the detection of fragment-length polymorphisms (FLPs) caused by InDels. The protocol utilizes standard sequencers and genotyping software. We have established genome-wide FLP maps for both Caenorhabditis elegans and Drosophila melanogaster that facilitate genetic mapping with a minimum of manual input and at comparatively low cost.
For humans and model organisms, such as worms and flies, the availability of high-density sequence polymorphism maps greatly facilitates the rapid mapping and cloning of genes [1–3]. Key advantages of most molecular polymorphisms are the fact that they are codominant and in general phenotypically neutral. The vast majority of sequence polymorphisms are single-nucleotide polymorphisms (SNPs).
The most direct approach for SNP detection is sequencing of a PCR product spanning the polymorphism, but this is too costly and labor intense for high-throughput genotyping. For this reason, several different strategies and methods have been developed in order to detect SNPs more efficiently. In general, assays can be grouped into strategies, where the nature of the SNP is determined by directly analyzing the primary PCR product and those that require a secondary assay performed on the primary amplification product [4–6]. An important strategy of the first group is the 5' nuclease assay, where allele-specific, dual-labeled fluorescent TaqMan probes guarantee specificity . However, the need for two dual-labeled fluorescent probes, expensive specialized chemistry and specialized machinery increase the costs per assay of this approach significantly. Similarly, denaturing high-performance liquid chromatography (DHPLC) also analyses the primary amplification product . This approach is based on melting differences of homo- versus heteroduplex DNA fragments under increasingly denaturing conditions and requires no specific labeling of the PCR fragments. However, conditions have to be optimized for every assay, throughput is limited and specialized equipment is required. DHPLC has been used in small-scale genotyping projects in Drosophila melanogaster .
Of the methods that detect the SNP in a secondary assay, restriction fragment length polymorphism (RFLP) analysis are very popular . For this purpose, only those SNPs that alter a restriction site are analyzed. A great advantage of RFLP analysis is that no specialized equipment is needed and it can be carried out in every laboratory. RFLP maps recently established for Caenorhabditis elegans and Drosophila are used regularly in genotyping projects [2, 3, 11]. However, RFLP analysis requires significant manual input. Moreover, the use of different restriction enzymes with different reaction requirements adds another level of complexity that makes this method difficult to automate. Primer-extension-based technologies have also gained some prominence . Here, a primer that anneals right next to the polymorphism is extended by one polymorphism-specific terminator nucleotide. Extension products are analyzed by size or, alternatively, by differences in the behavior of incorporated versus non-incorporated terminator nucleotides under polarized fluorescent light . Swan and colleagues  have developed a set of fluorescence polarization-template directed incorporation (FP-TDI) assays for C. elegans. However, this approach is labor intensive and requires specialized chemistry and equipment. Using DNA microarrays, large numbers of SNPs can be analyzed in parallel, but the number of individuals that can be analyzed is low because of the high cost per chip [15, 16].
Besides SNPs, short tandem repeats (STRs) or microsatellites represent another class of sequence polymorphisms used for genotyping [17–21]. STRs result in fragment length differences that are either detected on gel-based or capillary sequencers or high-resolution hydrogels (Elchrom Scientific Inc.). One advantage of STRs over SNPs is that they are highly polymorphic and are thus ideal for measuring the degree of variability in natural populations. STRs are, however, present at much lower density than SNPs and are therefore not suitable for high-resolution mapping of genes.
Interestingly, a significant proportion of the currently available polymorphisms are caused by small insertions or deletions (InDels). Weber et al.  identified a genome-wide set of about 2,000 human InDel polymorphisms and estimated that InDels comprise at least 8% and up to 20% of all human polymorphisms. This is in line with the findings of Berger and co-workers  who found that 16.2% of polymorphisms in Drosophila are of the InDel type. Also, two independent studies in C. elegans found that InDels constitute between 25% and 28% of all polymorphisms [3, 14]. In addition, those studies found that the vast majority of InDels are due to 1-2 base-pair (bp) differences (65% in Drosophila , 84% in C. elegans ).
To take full advantage of this class of small InDel polymorphisms, we have developed a strategy that allows us to detect most, if not all, InDels by analyzing the lengths of primary PCR products on a capillary sequencer at single base-pair resolution. We call these assays fragment length polymorphism (FLP) assays. Importantly, this approach can easily be automated on standard robotic pipetting platforms as it involves a simple PCR reaction setup. Furthermore, allele calling is performed automatically using the Applied Biosystems GeneMapper software commonly used for genotyping STRs (Materials and methods).
To demonstrate the feasibility of this strategy, we have validated 112 evenly spaced FLP assays at 3 centimorgan (cM) resolution in C. elegans (one every 0.9 megabase-pair (Mbp)) and 54 FLP assays at 4 cM resolution for the Drosophila autosomes. This set of FLP assays allows us to rapidly map mutations to small chromosomal subregions with a minimum of manual input. Furthermore, we provide a list of predicted InDels for which additional assays can be readily designed in the chromosomal subregion of interest. Those non-validated FLPs enhance the resolution of the map by a factor of 5.6 and 17.9, respectively.
We show the usefulness of this approach by identifying novel alleles of previously characterized genes. In summary, we have taken advantage of a publicly available dataset to adapt a technology widely used for STR analysis to genetic mapping. Thanks to the complete automation of genotyping, this approach is considerably faster, more reliable and cheaper than previously used mapping strategies in C. elegans or Drosophila.
Results and discussion
Detection of fragment length polymorphisms (FLPs)
To detect a FLP, the region of interest is amplified in a standard PCR reaction with one fluorescently labeled primer, and the PCR products are directly analyzed on a capillary sequencer. Fragment sizes are determined automatically relative to an internal size standard with AppliedBiosystem's GeneMapper software (for details see Materials and methods). The software then allocates fragment sizes to previously calibrated genotypes.
Genotyping with FLP assays is extremely accurate. In a control experiment, we genotyped all 96 samples of the fly strains FRT42B and EP0755 for the 1-bp InDel 2R090 and 231 samples homo- and heterozygous for the C. elegans Bristol and Hawaii backgrounds, respectively, for the 1-bp InDel ZH5-16. 2R090 exhibits both stuttering and A addition and hence is especially difficult to resolve (see Additional data file 8). The genotype was correctly and automatically assigned by GeneMapper in all 423 assays. Thus, automated genotyping based on FLPs is sensitive down to single base-pair resolution and is extremely robust. The accuracy of FLP mapping is comparable to other methods such as TaqMan (error rate less than 1 in 2,000 ), minisequencing (99.5% ), and pyrosequencing (97.3 % ).
C. elegans and DrosophilaFLP maps
To establish a Drosophila FLP map, a set of 54 FLP assays (12 to 17 per arm of the two major autosomes) was validated from the list of polymorphisms identified by Berger et al.  (Figure 2b, and Additional data file 10); high-resolution X-chromosomal SNP and FLP maps have yet to be established. Similarly to C. elegans, the confirmation rate of the predicted Drosophila InDels was 80% (n = 30). Furthermore, another 509 InDels are predicted at 248 sites for which an assay can be established to discriminate between EP and FRT strains (Additional data file 18). The validated Drosophila FLP assays were evenly spaced on the genetic map with an average distance between neighboring assays of about 4 cM, corresponding to an average resolution of 1.77 Mbp on the physical map encompassing 95,55 Mbp [27, 28]. Taking into account the non-validated InDels, the maximal average resolution is currently 314 kb or 0.7 cM. On the left arm of chromosome 3, where the genetic map is inexact, FLPs were spaced on the physical map assuming colinearity between the two maps. The length of amplicons ranges from 99 to 365 bp, and the size difference ranges from 1 to 54 bp (Additional data file 9).
Our Drosophila FLP assays are in part derived from a set of InDels of size difference 7 bp or more (termed PLPs by Berger et al. ). However, since 86.8% of all Drosophila InDels exhibit a length difference of one to six nucleotides , so far only a small subset of the available InDels has been covered. The approach presented here significantly increases the number of possible FLP assays for genotyping and offers a greater flexibility and higher resolution.
FLP mapping of C. elegansgenes
In cases where a mutation maps to an interval that contains no obvious candidate gene, we first screen for additional informative recombinants by FLP analysis and then refine the map position by extracting more FLPs from our set of non-validated InDels (Additional data files 12-17) and by genotyping existing SNPs in the candidate interval . In many cases, this resolution is sufficient to identify the affected gene through RNA interference (RNAi) analysis of the genes in the corresponding interval . (See Additional data file 6 for a detailed flowchart of the mapping process).
In summary, FLP mapping in C. elegans allows us to rapidly map a mutation down to a small region containing, on average, 200 candidate genes by crossing a mutant strain to CB4856 and analyzing 48 F2 animals with 300 to 500 PCR reactions.
Genotyping Drosophilastrains with FLP assays
In contrast to the well defined genetic backgrounds used for C. elegans, zebrafish (Danio rerio) or Arabidopsis genetics, Drosophila strains are very heterogeneous and of ill-defined origin [2, 9, 11]. In this respect, gene mapping in Drosophila resembles human genetics in that standard inbred lines do not exist and the genotypes of the parental lines have to be determined first. As genome-wide polymorphism databases for reference strains are available [2, 11], a line of interest can be crossed with two reference strains, such as EP and FRT (see below). Owing to the codominant character of sequence polymorphisms, at least one of the two respective crosses will distinguish between the mutant and the mapping chromosomes. To further facilitate mapping with our set of FLP assays, we genotyped several common laboratory lines such as two 'wild-type' yw strains for the whole set, four FRT-Minute or FRT-cell-lethal strains at the relevant autosomal arms , as well as the FRT and EP reference strains at both relevant autosomal arms (Figure 2b). Surprisingly, the FRT and EP lines are largely not of FRT or EP genotype on the chromosome arm for which they have not been calibrated. Overall, we found novel alleles for 18 of the 48 assays, and in an extreme case, we even observed five different alleles in five examined strains (2R017, Figure 2b). This result further highlights the heterogeneity of Drosophila strains (see Additional data file 1 for further details on FLP calibration and fly genetics).
FLP mapping in Drosophila
If the resolution of the validated FLP map is too low to identify a candidate gene, we further refine the map position by several approaches. First, we design novel FLP-assays in the region of interest and genotype the most informative recombinants from the first round of FLP mapping (Additional data file 18). Second, we genotype recombinants with SNPs available in the region of interest and resolve them by RFLP, sequencing or DHPLC [2, 9]. Third, we perform complementation analysis with recently established Drosophila lines with molecularly defined deletions [37, 38]. (See Additional data file 7 for a detailed flowchart illustrating the mapping process.)
We have developed an automated method to detect most naturally occurring InDel polymorphisms at single base-pair resolution. Since a significant fraction of polymorphisms are caused by InDels of only a few base pairs (for example, 8% to 20% in humans ) the resolution of the medium-density FLP maps can be greatly increased where necessary, for example during the positional cloning of genes. We are therefore continually designing new FLP assays according to our specific needs using the predicted FLPs (Additional data files 12-18). The full automation of the genotyping has three main advantages when compared to manual methods. First, the error rate (the number of wrongly assigned genotypes) is extremely low, as it was not measurable in 432 assays. Second, genotyping can be done very rapidly and at a high-throughput with little manpower. The automatic allele-calling, in particular, saves much time. As the identification of informative recombinants is usually the rate-limiting step, FLP mapping is very helpful in extracting the few relevant recombinants from a large number of samples. Third, thanks to the standardized conditions, the low error rate and the absence of a secondary assay, FLP mapping is considerably cheaper than the previously published 'manual' mapping methods [2, 3]. Unlike other high-throughput methods like TaqMan, Pyrosequencing, DHPLC, fluorescence polarization or primer-extension assays, FLP mapping does not require any investment in specialized equipment. It can be done in any molecular biology lab with access to a sequencing facility equipped with a capillary- or gel-based system, which usually includes the genotyping software. PCR costs are marginally higher because of the use of fluorescently labeled primers, but there are no added expenses for secondary enzymatic assays.
It seems likely that in most organisms the frequency of polymorphisms caused by InDels is in the same range as found in humans, C. elegans or Drosophila. For example, 7.3% of the Arabidopsis sequence polymorphisms are InDels . Thus, FLP mapping can easily be adapted to any organism for which polymorphism maps have been established, as there is no conceptual difference between human, Arabidopsis, C. elegans or Drosophila FLPs.
Materials and methods
C. elegans and Drosophilaculture techniques and alleles
Culturing and crossing of C. elegans was done according to standard procedures described in . C. elegans alleles used were: LG I: lin-11(zh41), lin-11(n389); LG II: rol-1(e91), let-23(sy1), unc-52(e444). Drosophila strains and the genetic screen have been described previously [9, 35, 40–42].
Single worm DNA extraction
Adult worms were collected in 10 μl lysis buffer (50 mM KCl, 10 mM Tris pH 8.2, 2.5 mM MgCl2, 0.45% NP-40, 0.45% Tween-20, 100 μg/ml freshly added proteinase K) and incubated for 60 min at 65°C followed by heat-inactivation of proteinase K at 95°C for 10 min. Before PCR, 90 μl double-distilled H2O (ddH2O) was added to obtain a total volume of 100 μl per lysate.
Fly DNA extraction
DNA from recombinant flies was extracted in bulk by squishing flies through mechanical force in a vibration mill (Retsch MM30) programmed to shake for 20 sec at 20 strokes per second . Single flies were placed into wells of a 96-well format deep-well plate with each well filled with 200 μl squishing buffer (10 mM Tris-Cl pH 8.2, 1 mM EDTA, 0.2% Triton X-100, 25 mM NaCl, 200 μg/ml freshly added proteinase K) and a tungsten carbide bead (Qiagen). The deep-well plate was then sealed with a rubber mat (Eppendorf) and clamped into the vibration mill. (Tungsten carbide beads can be recycled: after an overnight incubation in 0.1 M HCl and thorough washing in ddH2O the beads are virtually free of contaminating DNA.) Debris was allowed to settle for about 5 min, and 50 μl of each supernatant were transferred into a 96-well PCR plate. The reactions were incubated in a thermo-cycler for 30 min at 37°C and finally for 10 min at 95°C to heat-inactivate proteinase K. Before PCR amplification, the crude DNA extracts were diluted 20-fold to reduce the concentration of proteins that might be harmful for the capillary sequencer.
PCR and FLP fragment analysis
Diluted single-worm lysates (2 μl samples) or single fly extracts were added to 23 μl PCR reaction mix. Final concentrations in the PCR reaction were: 0.4 μM forward/reverse primer, 0.2 mM dNTPs, 2 mM MgCl2, 1x PCR reaction buffer, 0.25 U EuroTaq polymerase (Euroclone). PCR reaction setup was done in 96-well plates using a Tecan Genesis pipetting robot with disposable tips. PCR was carried out in two MJR thermo-cyclers that are integrated into the robot. The current setup allows for the sequential processing of six 96-well plates at a time. Cycling parameters were 2 min 95°C, 20 sec 95°C, 20 sec 61°C (-0.5°C for each cycle), 45 sec 72°C (for 10 cycles) followed by 24 cycles of 20 sec 95°C, 20 sec 56°C, 45 sec 72°C and a 10 min 72°C final extension. Following PCR, reactions were diluted 1:100 in water, and 2 μl diluted PCR products were mixed with 10 μl HiDi formamide containing 0.025 μl LIZ500 size standard (Applied Biosystems). This dilution before analysis on the capillary sequencer is necessary to reduce signal intensity because too strong signals compromise data analysis. In addition, sample dilution reduces the risk of damaging the capillaries with proteins or lipids present in the crude lysates. The dilution was done with standard tips using the Tecan Genesis pipetting station. Carryover of fragments was prohibited by a simple wash step with H2O. Fragments were analyzed on an ABI3730 capillary sequencer using POP7 polymer according to standard procedures. Data were analyzed using AppliedBiosystems GeneMapper software and raw data were treated further with Microsoft Excel.
Additional data files
The following additional data are available with the online version of this article. Additional data file 1 contains general information on fly genetics.
Further C. elegans mapping results are given in Additional data files 2,3,4 and 5. Detailed flowcharts illustrating the FLP mapping process are shown in Additional data files 6 and 7. Additional data file 8 contains electropherograms demonstrating the accuracy of allele-calling. Additional data files 9 and 10 contain tables of primer and sequence data of experimentally verified FLP assays in C. elegans and Drosophila, respectively. Additional data file 11 contains a table of the refined genetic distances for FLP assays on the right arm of Drosophila chromosome 2. Additional non-validated FLPs can be found in Additional data files 12,13,14,15,16 and 17 (C. elegans) and Additional data file 18 (Drosophila).
We are grateful to Carmen Rottig for providing us with the novel hippo mutant and to DJ Pan for the hpo42-20 mutation. Angela Baer is acknowledged for excellent technical assistance. This work was funded by projects from the Swiss National Science Foundation and the Kanton Zürich.
- Sachidanandam R, Weissman D, Schmidt SC, Kakol JM, Stein LD, Marth G, Sherry S, Mullikin JC, Mortimore BJ, Willey DL, et al: A map of human genome sequence variation containing 1.42 million single nucleotide polymorphisms. Nature. 2001, 409: 928-933. 10.1038/35057149.PubMedView ArticleGoogle Scholar
- Berger J, Suzuki T, Senti KA, Stubbs J, Schaffner G, Dickson BJ: Genetic mapping with SNP markers in Drosophila. Nat Genet. 2001, 29: 475-481. 10.1038/ng773.PubMedView ArticleGoogle Scholar
- Wicks SR, Yeh RT, Gish WR, Waterston RH, Plasterk RH: Rapid gene mapping in Caenorhabditis elegans using a high density polymorphism map. Nat Genet. 2001, 28: 160-164. 10.1038/88878.PubMedView ArticleGoogle Scholar
- Kwok PY, Chen X: Detection of single nucleotide polymorphisms. Curr Issues Mol Biol. 2003, 5: 43-60.PubMedGoogle Scholar
- Syvanen AC: Accessing genetic variation: genotyping single nucleotide polymorphisms. Nat Rev Genet. 2001, 2: 930-942. 10.1038/35103535.PubMedView ArticleGoogle Scholar
- Chen X, Sullivan PF: Single nucleotide polymorphism genotyping: biochemistry, protocol, cost and throughput. Pharmacogenomics J. 2003, 3: 77-96. 10.1038/sj.tpj.6500167.PubMedView ArticleGoogle Scholar
- Livak KJ: Allelic discrimination using fluorogenic probes and the 5' nuclease assay. Genet Anal. 1999, 14: 143-149.PubMedView ArticleGoogle Scholar
- Wolford JK, Blunt D, Ballecer C, Prochazka M: High-throughput SNP detection by using DNA pooling and denaturing high performance liquid chromatography (DHPLC). Hum Genet. 2000, 107: 483-487. 10.1007/s004390000396.PubMedView ArticleGoogle Scholar
- Nairz K, Stocker H, Schindelholz B, Hafen E: High-resolution SNP mapping by denaturing HPLC. Proc Natl Acad Sci USA. 2002, 99: 10575-10580. 10.1073/pnas.162136299.PubMedPubMed CentralView ArticleGoogle Scholar
- White R, Lalouel JM: Chromosome mapping with DNA markers. Sci Am. 1988, 258: 40-48.PubMedView ArticleGoogle Scholar
- Hoskins RA, Phan AC, Naeemuddin M, Mapa FA, Ruddy DA, Ryan JJ, Young LM, Wells T, Kopczynski C, Ellis MC: Single nucleotide polymorphism markers for genetic mapping in Drosophila melanogaster. Genome Res. 2001, 11: 1100-1113. 10.1101/gr.GR-1780R.PubMedPubMed CentralView ArticleGoogle Scholar
- Syvanen AC: From gels to chips: "minisequencing" primer extension for analysis of point mutations and single nucleotide polymorphisms. Hum Mutat. 1999, 13: 1-10.PubMedView ArticleGoogle Scholar
- Kwok PY: High-throughput genotyping assay approaches. Pharmacogenomics. 2000, 1: 95-100. 10.1517/14622418.104.22.168.PubMedView ArticleGoogle Scholar
- Swan KA, Curtis DE, McKusick KB, Voinov AV, Mapa FA, Cancilla MR: High-throughput gene mapping in Caenorhabditis elegans. Genome Res. 2002, 12: 1100-1105.PubMedPubMed CentralGoogle Scholar
- Sosnowski RG, Tu E, Butler WF, O'Connell JP, Heller MJ: Rapid determination of single base mismatch mutations in DNA hybrids by direct electric field control. Proc Natl Acad Sci USA. 1997, 94: 1119-1123. 10.1073/pnas.94.4.1119.PubMedPubMed CentralView ArticleGoogle Scholar
- Gilles PN, Wu DJ, Foster CB, Dillon PJ, Chanock SJ: Single nucleotide polymorphic discrimination by an electronic dot blot assay on semiconductor microchips. Nat Biotechnol. 1999, 17: 365-370. 10.1038/7921.PubMedView ArticleGoogle Scholar
- Weissenbach J: Microsatellite polymorphisms and the genetic linkage map of the human genome. Curr Opin Genet Dev. 1993, 3: 414-417. 10.1016/0959-437X(93)90114-5.PubMedView ArticleGoogle Scholar
- A comprehensive genetic linkage map of the human genome. NIH/CEPH Collaborative Mapping Group. Science. 1992, 258: 67-86.Google Scholar
- McCouch SR, Chen X, Panaud O, Temnykh S, Xu Y, Cho YG, Huang N, Ishii T, Blair M: Microsatellite marker development, mapping and applications in rice genetics and breeding. Plant Mol Biol. 1997, 35: 89-99. 10.1023/A:1005711431474.PubMedView ArticleGoogle Scholar
- Knapik EW, Goodman A, Ekker M, Chevrette M, Delgado J, Neuhauss S, Shimoda N, Driever W, Fishman MC, Jacob HJ: A microsatellite genetic linkage map for zebrafish (Danio rerio). Nat Genet. 1998, 18: 338-343. 10.1038/ng0498-338.PubMedView ArticleGoogle Scholar
- Collins JR, Stephens RM, Gold B, Long B, Dean M, Burt SK: An exhaustive DNA micro-satellite map of the human genome using high performance computing. Genomics. 2003, 82: 10-9. 10.1016/S0888-7543(03)00076-4.PubMedView ArticleGoogle Scholar
- Weber JL, David D, Heil J, Fan Y, Zhao C, Marth G: Human diallelic insertion/deletion polymorphisms. Am J Hum Genet. 2002, 71: 854-862. 10.1086/342727.PubMedPubMed CentralView ArticleGoogle Scholar
- Smith JR, Carpten JD, Brownstein MJ, Ghosh S, Magnuson VL, Gilbert DA, Trent JM, Collins FS: Approach to genotyping errors caused by nontemplated nucleotide addition by Taq DNA polymerase. Genome Res. 1995, 5: 312-317.PubMedView ArticleGoogle Scholar
- Ranade K, Chang MS, Ting CT, Pei D, Hsiao CF, Olivier M, Pesich R, Hebert J, Chen YD, Dzau VJ, et al: High-throughput genotyping with single nucleotide polymorphisms. Genome Res. 2001, 11: 1262-1268.PubMedPubMed CentralGoogle Scholar
- Chen DC, Saarela J, Nuotio I, Jokiaho A, Peltonen L, Palotie A: Comparison of GenFlex Tag array and pyrosequencing in SNP genotyping. J Mol Diagn. 2003, 5: 243-249.PubMedPubMed CentralView ArticleGoogle Scholar
- Brenner S: The genetics of Caenorhabditis elegans. Genetics. 1974, 77: 71-94.PubMedPubMed CentralGoogle Scholar
- Lindsley DL, Zimm GG: The genome of Drosophila melanogaster. 1992, New York: Academic PressGoogle Scholar
- Adams MD, Celniker SE, Holt RA, Evans CA, Gocayne JD, Amanatides PG, Scherer SE, Li PW, Hoskins RA, Galle RF, et al: The genome sequence of Drosophila melanogaster. Science. 2000, 287: 2185-2195. 10.1126/science.287.5461.2185.PubMedView ArticleGoogle Scholar
- Aroian RV, Sternberg PW: Multiple functions of let-23, a Caenorhabditis elegans receptor tyrosine kinase gene required for vulval induction. Genetics. 1991, 128: 251-267.PubMedPubMed CentralGoogle Scholar
- Higgins BJ, Hirsh D: Roller mutants of the nematode Caenorhabditis elegans. Mol Gen Genet. 1977, 150: 63-72.PubMedView ArticleGoogle Scholar
- Mackenzie JM, Garcea RL, Zengel JM, Epstein HF: Muscle development in Caenorhabditis elegans: mutants exhibiting retarded sarcomere construction. Cell. 1978, 15: 751-762. 10.1016/0092-8674(78)90261-1.PubMedView ArticleGoogle Scholar
- Burdine RD, Branda CS, Stern MJ: EGL-17(FGF) expression coordinates the attraction of the migrating sex myoblasts with vulval induction in C. elegans. Development. 1998, 125: 1083-1093.PubMedGoogle Scholar
- Gupta BP, Wang M, Sternberg PW: The C. elegans LIM homeobox gene lin-11 specifies multiple cell fates during vulval development. Development. 2003, 130: 2589-2601. 10.1242/dev.00500.PubMedView ArticleGoogle Scholar
- Kamath RS, Fraser AG, Dong Y, Poulin G, Durbin R, Gotta M, Kanapin A, LeBot N, Moreno S, Sohrmann M, et al: Systematic functional analysis of the Caenorhabditis elegans genome using RNAi. Nature. 2003, 421: 231-237. 10.1038/nature01278.PubMedView ArticleGoogle Scholar
- Newsome TP, Asling B, Dickson BJ: Analysis of Drosophila photoreceptor axon guidance in eye-specific mosaics. Development. 2000, 127: 851-860.PubMedGoogle Scholar
- Ryoo HD, Steller H: Hippo and its mission for growth control. Nat Cell Biol. 2003, 5: 853-855. 10.1038/ncb1003-853.PubMedView ArticleGoogle Scholar
- Ryder E, Blows F, Ashburner M, Bautista-Llacer R, Coulson D, Drummond J, Webster J, Gubb D, Gunton N, Johnson G, et al: The DrosDel collection: a set of P-element insertions for generating custom chromosomal aberrations in Drosophila melanogaster. Genetics. 2004, 167: 797-813. 10.1534/genetics.104.026658.PubMedPubMed CentralView ArticleGoogle Scholar
- Parks AL, Cook KR, Belvin M, Dompe NA, Fawcett R, Huppert K, Tan LR, Winter CG, Bogart KP, Deal JE, et al: Systematic generation of high-resolution deletion coverage of the Drosophila melanogaster genome. Nat Genet. 2004, 36: 288-292. 10.1038/ng1312.PubMedView ArticleGoogle Scholar
- Schmid KJ, Sorensen TR, Stracke R, Torjek O, Altmann T, Mitchell-Olds T, Weisshaar B: Large-scale identification and analysis of genome-wide single-nucleotide polymorphisms for mapping in Arabidopsis thaliana. Genome Res. 2003, 13: 1250-1257. 10.1101/gr.728603.PubMedPubMed CentralView ArticleGoogle Scholar
- Xu T, Rubin GM: Analysis of genetic mosaics in developing and adult Drosophila tissues. Development. 1993, 117: 1223-1237.PubMedGoogle Scholar
- Rorth P: A modular misexpression screen in Drosophila detecting tissue-specific phenotypes. Proc Natl Acad Sci USA. 1996, 93: 12418-12422. 10.1073/pnas.93.22.12418.PubMedPubMed CentralView ArticleGoogle Scholar
- St Johnston D: The art and design of genetic screens: Drosophila melanogaster. Nat Rev Genet. 2002, 3: 176-188. 10.1038/nrg751.PubMedView ArticleGoogle Scholar
- Nairz K, Zipperlen P, Dearolf C, Basler K, Hafen E: A reverse genetic screen in Drosophila using a deletion-inducing mutagen. Genome Biol. 2004, 5: R83-10.1186/gb-2004-5-10-r83.PubMedPubMed CentralView ArticleGoogle Scholar
- Francis R, Waterston RH: Muscle cell attachment in Caenorhabditis elegans. J Cell Biol. 1991, 114: 465-479. 10.1083/jcb.114.3.465.PubMedView ArticleGoogle Scholar
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