Large-scale insertional mutagenesis of a coleopteran stored grain pest, the red flour beetle Tribolium castaneum, identifies embryonic lethal mutations and enhancer traps
- Jochen Trauner†1,
- Johannes Schinko†2,
- Marcé D Lorenzen†3,
- Teresa D Shippy†4,
- Ernst A Wimmer2Email author,
- Richard W Beeman3,
- Martin Klingler1,
- Gregor Bucher2 and
- Susan J Brown4
© Trauner et al; licensee BioMed Central Ltd. 2009
Received: 24 June 2009
Accepted: 05 November 2009
Published: 05 November 2009
Given its sequenced genome and efficient systemic RNA interference response, the red flour beetle Tribolium castaneum is a model organism well suited for reverse genetics. Even so, there is a pressing need for forward genetic analysis to escape the bias inherent in candidate gene approaches.
To produce easy-to-maintain insertional mutations and to obtain fluorescent marker lines to aid phenotypic analysis, we undertook a large-scale transposon mutagenesis screen. In this screen, we produced more than 6,500 new piggyBac insertions. Of these, 421 proved to be recessive lethal, 75 were semi-lethal, and eight indicated recessive sterility, while 505 showed new enhancer-trap patterns. Insertion junctions were determined for 403 lines and often appeared to be located within transcription units. Insertion sites appeared to be randomly distributed throughout the genome, with the exception of a preference for reinsertion near the donor site.
A large collection of enhancer-trap and embryonic lethal beetle lines has been made available to the research community and will foster investigations into diverse fields of insect biology, pest control, and evolution. Because the genetic elements used in this screen are species-nonspecific, and because the crossing scheme does not depend on balancer chromosomes, the methods presented herein should be broadly applicable for many insect species.
During the past few years, the red flour beetle Tribolium castaneum has been developed into a powerful model organism suited for the study of short germ development, embryonic head and leg development, metamorphosis, cuticle metabolism, and other problems in insect biology. It is the first coleopteran species for which the genome sequence has become available . In-depth functional analysis of molecularly identified genes is enabled by the availability of germline transformation [2, 3] and systemic RNA interference that is splice-variant-specific  and feasible at all life stages [5–7]. Furthermore, several tools and techniques have been developed that facilitate insertional mutagenesis in Tribolium castaneum [8–11]. Although candidate gene approaches (reverse genetics) via RNA interference work very well in Tribolium, they are biased towards previously recognized genes and mechanisms. In contrast, forward genetic approaches offer the opportunity to detect new gene functions not yet described in other model systems. Small-scale chemical mutagenesis screens have been performed in Tribolium [12, 13], but stock-keeping of unmarked recessive mutants is difficult due to the number of chromosomes (n = 10) and the lack of balancers (< 50% of the genome is covered) . In contrast, insertional mutagenesis screens using dominantly-marked donor transposons facilitate both stock-keeping and gene identification.
Several species-nonspecific transposons including Hermes, Minos, and piggyBac have been shown to function in Tribolium [2, 10]. Berghammer et al.  introduced enhanced green fluorescent protein (EGFP) under the control of the 3xP3 promoter as a universal, selectable marker for transgenic insects. This promoter is also responsive to nearby chromosomal enhancers , allowing insertional mutagenesis to be combined with enhancer trapping . In our scheme, insertional mutagenesis is based on the controlled remobilization of a non-autonomous donor element stably inserted in the genome. The transposase needed to remobilize the donor element is provided by a helper element (jumpstarter). Lorenzen et al.  created several jumpstarter strains using a modified Minos transposon to provide a source of piggyBac transposase .
Here we report the first large-scale insertional mutagenesis screen conducted in an insect other than Drosophila. We have identified many insertion lines that are either homozygous lethal, homozygous sterile and/or show enhancer-trap patterns at various developmental stages. The genomic locations, enhancer-trap patterns (if present), recessive phenotypes, and genes affected by these transposon insertions are documented in the GEKU database (freely accessible at http://www.geku-base.uni-goettingen.de) and insertion lines are available upon request [GEKU: Göttingen, Erlangen, Kansas State University (KSU), United States Department of Agriculture (USDA)].
Our screening procedure should be applicable to many other insect species, because all genetic elements (transposons, promoters and marker genes) used in this screen are species-nonspecific . It also renders unnecessary the use of balancer chromosomes, which are not available for the vast majority of insect species. Obvious limitations may be the ability to rear the insect species in the laboratory, the feasibility of germline transformation to obtain donor and helper strains, and the ability to perform single-pair matings with high efficiency.
Test for lethality and sterility
Results of lethality/sterility test (F3 cross)
First round of single-pair matings
Second round of single-pair matings
number of insertions
number of insertions
Potentially homozygous sterile insertions lines were identified by evaluating the single-pair matings: Whenever two or more of the initial single-pair F3 self-crosses (round one, Figure 1E) failed to produce offspring (although the parents were alive and healthy), the line was classified as potentially sterile. This was the case for 160 insertions (Table 1). We used either of two methods to confirm or refute a tentative diagnosis of recessive sterility. In the first method, we set up a second round of single-pair self-crosses bringing the total number of F3 crosses to 20. The diagnosis was considered to be corroborated when the number of single-pair matings not producing any offspring increased to four or more. Using this definition, 124 potentially sterile lines were reduced to 21. However, further testing of these presumably sterile insertion lines showed that this criterion was not always reliable (see below). In the second method we set up 10 male and 10 female outcrosses. The diagnosis of recessive sterility was considered to be corroborated if the crosses failed to reveal either a fertile, homozygous male or a fertile, homozygous female. Out of 36 potentially sterile lines tested by the second method, only eight lines fulfilled this definition of sterility. Since the second follow-up test appeared to be more rigorous than the first, we retested 11 of the 21 apparently sterile lines from the former test using the more rigorous criterion. All 11 lines proved to be fertile in both sexes. It seems to be clear that most sterile lines found by using the first criterion are false-positives. Hence, we suggest using the stricter test for recessive sterility, which has the added benefit of identifying the affected sex.
Detection of enhancer traps
Analysis of lethal lines and developmental phenotypes
We analyzed the embryonic cuticle phenotypes of many lines identified as lethal and found a number of distinct cuticular abnormalities (Figure 2I-L). For example, line G08519 displays a phenotype similar to the proboscipedia ortholog maxillopedia in that maxillary (grey arrows) and labial (white arrow) palps are transformed to legs (Figure 2J); [16, 17]. Indeed, this insertion is located in the first intron of maxillopedia. In addition, many lethal lines showed a high proportion of embryos that died prior to cuticularization, indicating early embryonic lethality.
To test whether the semi-lethal lines are false positives or true lethals with occasional escapers, we checked what portion of these lines (Göttingen subset) produce lethal L1 cuticle phenotypes (at least two cuticles with similar strong defects in one preparation when scoring at least 10 individuals) and compared it to the percentage of cuticle phenotypes produced by the other classes. A total of 25.8% (8/31) of a random selection of lines complying with the strict definition of lethality showed such phenotypes. Of lines with one or two single-pair matings (out of 20) indicating homozygosity (semi-lethality), this portion was 16.6% in each case (5/30 and 3/18, respectively). Lines with three single-pair matings indicating homozygous viability gave rise to cuticle phenotypes in only 6.25% (1/16). Thus analyzing semi-lethal lines led to the identification of additional cuticle phenotype-inducing mutations.
Chromosomal location of new piggyBacinsertions
Chromosomal location of lethal piggyBac insertions
Chromosome size* [Mb]
The GEKU insertional mutagenesis screen was designed to meet the following criteria: It should be rapid and simple (i.e. involve as few generations as possible); and the analysis of the resulting insertion lines should be highly efficient (i.e. producing only a small number of false positive lethal or sterile lines, while also minimizing the frequency of false negatives; see Methods).
Large-scale insertional mutagenesis is feasible in a coleopteran species
Based on a pilot screen published in Lorenzen et al.  we have performed the first high-efficiency, large-scale insertional mutagenesis screen in an insect species outside the genus Drosophila, and we have established a crossing scheme that circumvents the need for balancer chromosomes or embryo injections. From our experience, we estimate that using the procedure presented here, one person should be able to establish 150 lethal strains per year. While the GEKU screen has identified many interesting enhancer traps and lethal phenotypes, genome-wide saturation would be difficult to achieve at the current level of efficiency. The most time-consuming step is setting up and evaluating 20 single-pair matings for each new insertion line to detect recessive lethality. For this reason we set up a small number of single-pair matings first, as most viable insertions can be identified by evaluating just a few crosses from each subset. However, also for insertions recognized as viable it was important to assess the fertility of all remaining single-pair matings in order to ensure that recessive sterile insertions were detected.
Lethal insertions are readily detected while insertions causing sterility are difficult to detect
We found that lethal lines were readily detected by single-pair matings. Based on the frequency with which semi-lethal lines produced strong L1 larval cuticle phenotypes, we suggest defining lines as potentially lethal when only one or two out of 20 single-pair matings indicate homozygosity. However, our definition of sterility proved to be too lax in the beginning, since most potentially sterile lines turned out to be false-positives in more detailed analysis.
Comparing efficiencies with Drosophila melanogasterinsertional mutagenesis and enhancer-trap screens
The efficiency of generating lethal mutations by piggyBac-based insertional mutagenesis in Tribolium (7.4%) is similar to equivalent screens in Drosophila based either on piggyBac [9, 18] or P elements [19–21]. Whether the efficacy of such screens can potentially be doubled by the inclusion of splice acceptor sites or insulator sequences within the mutator element - as has been shown in Drosophila  - still has to be determined in Tribolium.
The enhancer detection rate within this large-scale insertional mutagenesis screen was also 7.4%. This is actually higher than in a comparable Drosophila screen where enhancer detection without a suitable amplification system was about 2% . Only after including a GAL4-based amplifier system could Drosophila enhancer detection be raised to 50% . However, such directed expression systems still need to be further developed and assayed in Tribolium before they can be used in insertional mutagenesis screens.
Correlation of phenotype (lethality, sterility, enhancer trap) with insertion site proximity to protein coding sequences (CDS)
Detailed analysis of lethal piggyBac insertion sites
< 500 bp**
500 bp - 2500 bp**
distant (> 2500 bp)**
seq or blast problem
Ways to enhance overall efficiency
In the described scheme, when new crosses were set up, one had to switch between fluorescence (to detect the transformation marker) and normal light (to determine sex) several times, which was a time-consuming procedure. To improve this situation considerably, we constructed and are testing new donors that use rescue of eye color by vermilion + as an indication of transformation [23, 24]. The use of such a system will also facilitate stock-keeping.
Another way to enhance efficiency in future screens might be the establishment of donors that include an artificial maternal-effect selfish element, e.g. Medea [[25, 26], see also Methods]. Such elements induce the death of all offspring of a female (maternal-lethal effect) except for those that have inherited the element (zygotic rescue). For example, a modified piggyBac donor element could incorporate a Medea element in tandem with the 3xP3-EGFP-marker. This modified donor element would be inserted at a chromosomal location tightly linked to an easily-scored recessive marker, such as the body-color mutation black . In the P1 cross this donor strain (homozygous for wild-type body color) would be mated with a helper strain (homozygous mutant for black). The resulting P2 animals would carry one copy each of the helper, the donor and the mutant black allele. Moreover, the latter two would be located in trans at similar positions on homologous chromosomes. Such P2 hybrids would be mated with beetles that were trans-heterozygous for black and the Medea-containing donor element, or, if the P2 hybrid is female, they could instead be mated to homozygous black (non-helper, non-Medea) males. F1 offspring with black body-color then would arise only if they inherit the black chromosome from both parents. Because the Medea-tagged donor is arranged in trans with black, such black offspring do not carry a donor, and hence lack zygotic rescue activity of the Medea element. This leads to their death by the maternal-lethal effect of the element. Only if the donor has been remobilized to another genomic location can offspring carry both black alleles as well as the rescuing donor. Hence, black body-color in the offspring indicates a remobilization event. This design would be an elegant means to enhance the detection of new insertion lines by obviating the need for fluorescence detection. It would also simplify the stock-keeping of lethal insertions, since a Medea element tightly linked with the lethal insertion would constitute a type of balanced lethal.
We have successfully established a method to conduct large-scale insertional mutagenesis screens in the beetle Tribolium castaneum. Using this method, we obtained several hundred lethal insertions as well as insertions producing enhancer-trap phenotypes. These lines have been made available to the research community.
The donor strain used in this screen, Pig-19, carries a 3xP3-EGFP marked piggyBac element, pBac [3xP3-EGFPaf], that confers both, insertion-site-independent eye-specific EGFP expression, and donor-site-dependent muscle-specific EGFP expression . We previously demonstrated that remobilization of the Pig-19 insertion results in G1 beetles lacking muscle-specific expression, but retaining eye-specific expression [3, 11]. Thus, the loss of muscle-specific expression can be used to detect remobilization events. The jumpstarter/helper strain used in this screen, M26 , carries an X-chromosomal insertion of a 3xP3-DsRed marked Minos element (pMi [3xP3-DsRed; Dm'hsp70-pBac]) . Both strains are in a white-eyed pearl mutant background to facilitate detection of eye-specific fluorescence.
Generating new piggyBacinsertions
We used a P1, P2 and F1 to F4 scheme to comply with the nomenclature of standard Drosophila F1 and F3 genetic screens, respectively (Figure 1). Donor remobilization occurred in the germline of the P2 generation, while new insertions and mutant homozygotes first appeared in the F1 and F3 generations, respectively. All crosses were carried out at 30-32°C. Virgin females were collected as pupae and stored at 23°C for up to six weeks prior to use. Insertional mutagenesis is described in detail in . In summary, P1 mass-matings were set up between donor males and helper females (Figure 1A) and subcultured at intervals of two to three weeks. P2 offspring were collected as pupae and examined to verify the presence of both piggyBac-based donor (EGFP marker) and Minos-based helper (DsRed marker) constructs. Individual P2 virgin females were outcrossed to three pearl males each to ensure insemination (Figure 1B). The piggyBac donor element can be remobilized by piggyBac transposase activity in the germ line of the hybrid. New insertions were recognized in the F1 progeny by the loss of donor-site-dependent EGFP expression (i.e. muscle fluorescence) coupled with retention of insertion-site-independent EGFP expression (i.e. eye fluorescence). For each P2 outcross, a single F1 beetle carrying a new insertion was outcrossed once again to pearl to check for single insertions (based on 50% Mendelian segregation of the new insert) and to generate families for subsequent analysis. For stability of the new insertions, only individuals carrying a new insertion and lacking the helper element (i.e. DsRed negative) were chosen (Figure 1C). Additionally, depending on the new chromosomal location of piggyBac, a new insertion might show a novel enhancer-trap pattern. Even when a P2 cross produced multiple EGFP-positive offspring, only one F1 beetle was chosen for continued study in order to ensure independent origin of each new insertion. This was necessary because several offspring carrying the same insertion could appear within a P2 family as a result of a premeiotic remobilization event. For each F1 outcross, five female and three male F2 siblings were crossed to each other to establish new insertion strains and to enable testing for homozygous viability (F2 cross; Figure 1D). To accomplish the latter, we performed a number of single-pair F3 matings (Figure 1E) and analyzed their progeny for the presence of the donor element (see below).
Evaluation of F3 single-pair matings
Offspring of a single-pair mating
No offspring, but parents alive at the time of evaluation
Indicates sterility of one or both parents
No offspring, but one or both parents dead at the time of evaluation
uninformative single-pair mating*
At least one EGFP-negative progeny
This indicates heterozygosity of both parents.
All progeny EGFP positive, at least 20 beetles present
This indicates homozygosity of one or both parents
All progeny EGFP positive, but less than 20 beetles present
uninformative single-pair mating*
Test for lethality and sterility
First round of F3 single-pair matings (SPM)
Second round of F 3 single-pair matings (SPM)
At least one SPM indicates homozygosity
At least one SPM (in total) indicates homozygosity
All informative* SPM indicate heterozygosity of both parents
All informative* SPM indicate heterozygosity of both parents
At least two SPM without any offspring but with living parents
Unable to find at least four SPM (in total) without any offspring but with living parents (method 1) OR unable to identify either a fertile homozygous female or a fertile homozygous male (method 2)
The following potential errors could occur using this method to test for recessive lethality: (1) A homozygous-viable insertion mutant could be falsely judged homozygous lethal because all single-pair matings produced mixed progeny. This could occur if, by chance, all single-pair matings consisted of heterozygous beetles. The probability of such an occurrence is (2/3)n (n = number of beetles tested), because two-thirds of all EGFP-positive F3 beetles carrying a viable insertion are heterozygous. For eight single-pair matings (number of test beetles = 16), this probability equals 0.15%. For 20 single-pair matings, the probability that all (40) test beetles selected from a homozygous-viable line are heterozygous, is only 9.0 × 10-6. Thus, evaluating 20 single-pair matings is sufficient to exclude false-positive lethal lines with a very high level of confidence. (2) A homozygous-lethal insertion (all F2 progeny are heterozygous) could be falsely identified as homozygous viable if, by chance, no EGFP-negative progeny are observed from a single-pair mating, even though 25% are expected. The probability of this happening when 20 progeny are analyzed is about 0.3% (0.75n; n = number of progeny screened). Because the probability of misdiagnosing a lethal insertion rises if fewer progeny are analyzed, single-pair matings yielding less than 20 progeny were not used to make inferences about the lethality of the insertion (= 'uninformative single-pair mating' in Table 4) unless some progeny were EGFP negative.
Overcoming a negative X-chromosome bias
The fact that the helper insertion used in this work is X-linked imposed restrictions on the design of our crossing scheme. X-chromosomal insertions that were homozygous lethal or sterile could be obtained only if the following is considered: Because only new transformants that segregated away from the helper element were selected, hybrid females had to be used to set up P2 crosses in order to avoid bias against new X-linked insertions. Additionally, males with a new hemizygous X-linked lethal insertion would not survive and ones hemizygous for a new X-linked sterile insertion would be useless for generating a new stock. Hence, one could obtain X-linked lethal and sterile insertions only if female beetles carrying the donor element were used to set up the P2 as well as the F1 crosses. Therefore, we selected only female hybrids and used females carrying new insertions whenever possible.
Efficiency of detecting new insertions
At least one new insertion was detected in about 30% of all P2 crosses when about 20 offspring were screened. The percentage of P2 crosses that yield new insertions can be greatly increased by screening a larger number of progeny per P2 cross. For a subset of P2 crosses we screened 100 progeny per cross, and found at least one new insertion in every case. In practice, about 10 - 30 P2 pupae were present when the P2 progeny were screened for new insertions. The decision to discard the larval P2 offspring when a new insertion could not be detected in the first attempt represented a compromise between the need to find at least one new insertion in each family and the aim to obtain a large number of independent insertions with limited resources in time and space.
Determination of insertion sites
The genomic location of an insertion was determined by sequencing flanking DNA obtained by one of the following three polymerase chain reaction (PCR) -based methods: inverse PCR , universal PCR [3, 29], or vectorette PCR . The procedure for inverse PCR including primer design was adapted from 'Inverse PCR and Sequencing Protocol on 5 Fly Preps', Exelixis Pharmaceutical Corp (South San Francisco, California, USA) . Following DNA isolation, approximately 1 μg of DNA was digested with Sau3A1, BfUC1, or Ase1 (for 5' iPCR) or HinP1 (for 3' iPCR). Approximately 100 ng of digested DNA was then self-ligated to obtain circular DNA fragments, followed by two rounds of nested PCR. DNA templates (PCR products and/or cloned PCR products) were sequenced by Seqlab (Göttingen, Germany), Macrogen (Seoul, Korea), or using an ABI 3730 DNA sequencer (Sequencing and Genotyping Facility, Plant Pathology, Kansas State University, Manhattan, Kansas, USA). Data analysis was performed using Vector NTI® software (Invitrogen, Carlsbad, California, USA). After trimming vector sequences, flanking DNA sequences were then searched (BLASTN) against Tribolium castaneum genome sequences at HGSC, Baylor College of Medicine http://www.hgsc.bcm.tmc.edu/projects/tribolium/, NCBI http://www.ncbi.nlm.nih.gov/genome/seq/BlastGen/BlastGen.cgi?taxid=7070 or BeetleBase http://beetlebase.org/. If the insertion was in a predicted gene (GLEAN set), a transcription unit (EST or cDNA) or region indicated by Drosophila BLAST or other gene prediction method as a potential gene, the predicted Tribolium gene was examined by BLAST analysis at FlyBase for the top Drosophila hit, and NCBI (nr database) to identify other potential orthologs. Insertion site sequences were deposited to NCBI (for accession numbers see Additional File 1) and also put - including the retrieved information - into GEKU-base (see below).
Medea(maternal effect dominant embryonic arrest)
When hybrid females and pearl males (P2 generation) were crossed severe segregation distortion was observed: 98% of the progeny were EGFP positive, rather than the expected 50%. The DsRed marker however showed the expected 1:1 ratio (i.e. segregated independently of the EGFP marker). The unusual segregation of EGFP has been shown  to be the result of close cis-linkage (approximately 2 cM) of the maternally acting selfish gene Medea  with the Pig-19 donor insertion  on LG3. However, the segregation ratios of new insertions were affected only when the piggyBac element reinserted near the original donor insertion (representing a local hop).
All available information about the analyzed insertion lines can be found at a web-based database called GEKU-base http://www.geku-base.uni-goettingen.de. Information provided includes (if available) photographs and descriptions of enhancer traps and phenotypes, flanking sequences and chromosomal location, affected genes and their orthologs. GEKU-base also provides information on how to obtain insertion lines.
EGFP and DsRed analysis
Marker-gene fluorescence was detected using a Nikon fluorescence stereomicroscope SMZ1500 (Nikon GmbH, Düsseldorf, Germany) at Göttingen and Erlangen, an Olympus SZX12 fluorescence stereomicroscope (Olympus Corporation, Tokyo, Japan), or a Leica MZ FLIII fluorescence stereomicroscope (Leica Microsystems Inc., Wetzlar, Germany). The filter sets used for EGFP expression were: [Göttingen: 470/40 nm excitation filter, 500 nm LP emission filter, and 495 nm beamsplitter], [Erlangen: 480/40 nm excitation filter, 510 nm emission filter, and 505 nm beamsplitter], [KSU: 480/40 nm excitation filter and 535/50 nm emission filter], [USDA: GFP Plus filter set (excitation filter: 480/40 nm, barrier filter: 510 nm)]. The filter sets used for DsRed expression were: [Göttingen: 546/12 nm excitation filter, 605/75 nm emission filter, and 560 nm beamsplitter], [Erlangen: 565/30 excitation filter, 620/60 nm emission filter, and 585 nm beamsplitter], [KSU: 545/30 excitation filter and 620/60 emission filter], [USDA: TXR TEXAS RED filter set (excitation filter: 560/40 nm, barrier filter: 610 nm)]. To detect enhancer-trap patterns in embryos, we dechorionated embryos derived from F3-crosses.
Location of insertion lines shown in Figure 2
Gene names refer to respective Drosophila orthologs. The line E00321 is homozygous lethal and carries an insertion in lethal (2) giant larvae (Figure 2A). The line E00713 is homozygous viable and carries an insertion 149-bp upstream of the 5' end of GLEAN_03347, Glutatione S transferase, (Figure 2B). The homozygous viable line G01004 carries an insertion near Ultrabithorax (Figure 2C). The homozygous viable line G04717 carries an insertion near lame duck (Figure 2D). The line KT1539 is homozygous lethal and the insertion site is near the gene pointed (Figure 2E). The homozygous lethal line KS030 bears an insertion in an intron of lozenge (Figure 2F). The KS406 line is homozygous viable and carries an insertion in an intron of GLEAN_00277 which shows similarity to genes encoding protein tyrosine phosphatases. Other genes in the vicinity of this insertion are Fgf8 or Or48 (Figure 2G). The homozygous viable line MH30a has an insertion near female sterile (2) Ketel (Figure 2H). The line E00916 is homozygous lethal and carries an insertion in an exon of GLEAN_08270 (Drosophila ortholog: Cyclin D) (Figure 2I). The G08519 insertion is located in the first intron of proboscipedia (Figure 2J). The KT1096 insertion is in an intron of the pecanex ortholog (Figure 2K). The E03501 insertion is in an intron of the Tribolium ortholog of Ftz-F1 (Figure 2L).
enhanced green fluorescent protein
Göttingen, Erlangen, KSU, USDA
Kansas State University
first larval stage
maternal arrest dominant embryonic arrest
United States Department of Agriculture
We are deeply indebted to Elke Küster, Susanne Fischer, Tatum Kimzey, Kathy Leonard and Jonna Voorhees for technical assistance in production and characterization of transgenic lines. All programs and services of the U.S. Department of Agriculture are offered on a nondiscriminatory basis, without regard to race, color, national origin, religion, sex, age, marital status or handicap. Mention of trade names or commercial products in this publication is solely for the purpose of providing specific information and does not imply recommendation or endorsement by the USDA. This work has been funded by the USDA within the CSREES_NRI program "Functional Genomics of Agriculturally Important Organisms - Insects and Mites" grant #2004-35604-14250 (EAW, RWB, MK, SJB).
- Tribolium Genome Sequencing Consortium, Richards S, Gibbs RA, Weinstock GM, Brown SJ, Denell R, Beeman RW, Bucher G, Friedrich M, Grimmelikhuijzen CJ, Klingler M, Lorenzen M, Roth S, Schröder R, Tautz D, Zdobnov EM, Muzny D, Attaway T, Bell S, Buhay CJ, Chandrabose MN, Chavez D, Clerk-Blankenburg KP, Cree A, Dao M, Davis C, Chacko J, Dinh H, Dugan-Rocha S, Fowler G, Garner TT, et al: The genome of the model beetle and pest Tribolium castaneum. Nature. 2008, 452: 949-955. 10.1038/nature06784.View ArticleGoogle Scholar
- Berghammer AJ, Klingler M, Wimmer EA: A universal marker for transgenic insects. Nature. 1999, 402: 370-371. 10.1038/46463.View ArticlePubMedGoogle Scholar
- Lorenzen MD, Berghammer AJ, Brown SJ, Denell RE, Klingler M, Beeman RW: piggyBac-mediated germline transformation in the beetle Tribolium castaneum. Insect Mol Biol. 2003, 12: 433-440. 10.1046/j.1365-2583.2003.00427.x.View ArticlePubMedGoogle Scholar
- Arakane Y, Muthukrishnan S, Kramer KJ, Specht CA, Tomoyasu Y, Lorenzen MD, Kanost M, Beeman RW: The Tribolium chitin synthase genes TcCHS1 and TcCHS2 are specialized for synthesis of epidermal cuticle and midgut peritrophic matrix. Insect Mol Biol. 2005, 14: 453-463. 10.1111/j.1365-2583.2005.00576.x.View ArticlePubMedGoogle Scholar
- Brown SJ, Mahaffey JP, Lorenzen MD, Denell RE, Mahaffey JW: Using RNAi to investigate orthologous homeotic gene function during development of distantly related insects. Evol Dev. 1999, 1: 11-15. 10.1046/j.1525-142x.1999.99013.x.View ArticlePubMedGoogle Scholar
- Bucher G, Scholten J, Klingler M: Parental RNAi in Tribolium (Coleoptera). Curr Biol. 2002, 12: R85-86. 10.1016/S0960-9822(02)00666-8.View ArticlePubMedGoogle Scholar
- Tomoyasu Y, Denell RE: Larval RNAi in Tribolium (Coleoptera) for analyzing adult development. Dev Genes Evol. 2004, 214: 575-578. 10.1007/s00427-004-0434-0.View ArticlePubMedGoogle Scholar
- Horn C, Schmid BGM, Pogoda FS, Wimmer EA: Fluorescent transformation markers for insect transgenesis. Insect Biochem Mol Biol. 2002, 32: 1221-1235. 10.1016/S0965-1748(02)00085-1.View ArticlePubMedGoogle Scholar
- Horn C, Offen N, Nystedt S, Häcker U, Wimmer EA: piggyBac-based insertional mutagenesis and enhancer detection as a tool for functional insect genomics. Genetics. 2003, 163: 647-661.PubMed CentralPubMedGoogle Scholar
- Pavlopoulos A, Berghammer AJ, Averof M, Klingler M: Efficient Transformation of the Beetle Tribolium castaneum Using the Minos Transposable Element: Quantitative and Qualitative Analysis of Genomic Integration Events. Genetics. 2004, 167: 737-746. 10.1534/genetics.103.023085.PubMed CentralView ArticlePubMedGoogle Scholar
- Lorenzen MD, Kimzey T, Shippy TD, Brown SJ, Denell RE, Beeman RW: piggyBac-based insertional mutagenesis in Tribolium castaneum using donor/helper hybrids. Insect Mol Biol. 2007, 16: 265-275. 10.1111/j.1365-2583.2007.00727.x.View ArticlePubMedGoogle Scholar
- Sulston IA, Anderson KV: Embryonic patterning mutants of Tribolium castaneum. Development. 1996, 122: 805-814.PubMedGoogle Scholar
- Maderspacher F, Bucher G, Klingler M: Pair-rule and gap gene mutants in the flour beetle Tribolium castaneum. Dev Genes Evol. 1998, 208: 558-568. 10.1007/s004270050215.View ArticlePubMedGoogle Scholar
- Berghammer AJ, Bucher G, Maderspacher F, Klingler M: A system to efficiently maintain embryonic lethal mutations in the flour beetle Tribolium castaneum. Dev Genes Evol. 1999, 209: 382-389. 10.1007/s004270050268.View ArticlePubMedGoogle Scholar
- Horn C, Jaunich B, Wimmer EA: Highly sensitive, fluorescent transformation marker for Drosophila transgenesis. Dev Genes Evol. 2000, 210: 623-629. 10.1007/s004270000111.View ArticlePubMedGoogle Scholar
- Shippy TD, Brown SJ, Denell RE: Maxillopedia is the Tribolium ortholog of proboscipedia. Evol Dev. 2000, 2: 145-151. 10.1046/j.1525-142x.2000.00055.x.View ArticlePubMedGoogle Scholar
- Shippy TD, Guo J, Brown SJ, Beeman RW, Denell RE: Analysis of maxillopedia expression pattern and larval cuticular phenotype in wild-type and mutant Tribolium. Genetics. 2000, 155: 721-731.PubMed CentralPubMedGoogle Scholar
- Häcker U, Nystedt S, Barmchi MP, Horn C, Wimmer EA: piggyBac-based insertional mutagenesis in the presence of stably integrated P elements in Drosophila. Proc Natl Acad Sci USA. 2003, 100: 7720-7725. 10.1073/pnas.1230526100.PubMed CentralView ArticlePubMedGoogle Scholar
- Cooley L, Kelley R, Spradling A: Insertional mutagenesis of the Drosophila genome with single P elements. Science. 1988, 239: 1121-1128. 10.1126/science.2830671.View ArticlePubMedGoogle Scholar
- Bellen HJ: Ten years of enhancer detection: lessons from the fly. Plant Cell. 1999, 11: 2271-2281. 10.1105/tpc.11.12.2271.PubMed CentralView ArticlePubMedGoogle Scholar
- Peter A, Schöttler P, Werner M, Beinert N, Dowe G, Burkert P, Mourkioti F, Dentzer L, He Y, Deak P, Benos PV, Gatt MK, Murphy L, Harris D, Barrell B, Ferraz C, Vidal S, Brun C, Demaille J, Cadieu E, Dreano S, Gloux S, Lelaure V, Mottier S, Galibert F, Borkova D, Miñana B, Kafatos FC, Bolshakov S, Sidén-Kiamos I, et al: Mapping and identification of essential gene functions on the X chromosome of Drosophila. EMBO Rep. 2002, 3: 34-38. 10.1093/embo-reports/kvf012.PubMed CentralView ArticlePubMedGoogle Scholar
- Thibault ST, Singer MA, Miyazaki WY, Milash B, Dompe NA, Singh CM, Buchholz R, Demsky M, Fawcett R, Francis-Lang HL, Ryner L, Cheung LM, Chong A, Erickson C, Fisher WW, Greer K, Hartouni SR, Howie E, Jakkula L, Joo D, Killpack K, Laufer A, Mazzotta J, Smith RD, Stevens LM, Stuber C, Tan LR, Ventura R, Woo A, Zakrajsek I, et al: A complementary transposon tool kit for Drosophila melanogaster unsing P and piggyBac. Nature Genetics. 2004, 36: 283-287. 10.1038/ng1314.View ArticlePubMedGoogle Scholar
- Lorenzen MD, Brown SJ, Denell RE, Beeman RW: Cloning and characterization of the Tribolium castaneum eye-color genes encoding tryptophan oxygenase and kynurenine 3-monooxygenase. Genetics. 2002, 160: 225-234.PubMed CentralPubMedGoogle Scholar
- Lorenzen MD, Brown SJ, Denell RE, Beeman RW: Transgene expression from the Tribolium castaneum Polyubiquitin promoter. Insect Mol Biol. 2002, 11: 399-407. 10.1046/j.1365-2583.2002.00349.x.View ArticlePubMedGoogle Scholar
- Beeman RW, Friesen KS, Denell RE: Maternal-effect selfish genes in flour beetles. Science. 1992, 256: 89-92. 10.1126/science.1566060.View ArticlePubMedGoogle Scholar
- Chen CH, Huang H, Ward CM, Su JT, Schaeffer LV, Guo M, Hay BA: A synthetic maternal-effect selfish genetic element drives population replacement in Drosophila. Science. 2007, 316: 597-599. 10.1126/science. 1138595.View ArticlePubMedGoogle Scholar
- Sokoloff A, Slatis HM, Stanley J: The black mutation in Tribolium castaneum. J Heredity. 1960, 52: 131-135.Google Scholar
- Ochman H, Gerber AS, Hartl DL: Genetic applications of an inverse polymerase chain reaction. Genetics. 1988, 120: 621-623.PubMed CentralPubMedGoogle Scholar
- Beeman RW, Stauth DM: Rapid cloning of insect transposon insertion junctions using 'universal' PCR. Insect Mol Biol. 1997, 1: 83-88. 10.1046/j.1365-2583.1997.00159.x.View ArticleGoogle Scholar
- Arnold C, Hodgson I: Vectorette PCR: a novel approach to genomic walking. PCR Meth Appl. 1991, 1: 39-42.View ArticleGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.