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Technology transfer from worms and flies to vertebrates: transposition-based genome manipulations and their future perspectives
Genome Biology volume 8, Article number: S1 (2007)
To meet the increasing demand of linking sequence information to gene function in vertebrate models, genetic modifications must be introduced and their effects analyzed in an easy, controlled, and scalable manner. In the mouse, only about 10% (estimate) of all genes have been knocked out, despite continuous methodologic improvement and extensive effort. Moreover, a large proportion of inactivated genes exhibit no obvious phenotypic alterations. Thus, in order to facilitate analysis of gene function, new genetic tools and strategies are currently under development in these model organisms. Loss of function and gain of function mutagenesis screens based on transposable elements have numerous advantages because they can be applied in vivo and are therefore phenotype driven, and molecular analysis of the mutations is straightforward. At present, laboratory harnessing of transposable elements is more extensive in invertebrate models, mostly because of their earlier discovery in these organisms. Transposons have already been found to facilitate functional genetics research greatly in lower metazoan models, and have been applied most comprehensively in Drosophila. However, transposon based genetic strategies were recently established in vertebrates, and current progress in this field indicates that transposable elements will indeed serve as indispensable tools in the genetic toolkit for vertebrate models. In this review we provide an overview of transposon based genetic modification techniques used in higher and lower metazoan model organisms, and we highlight some of the important general considerations concerning genetic applications of transposon systems.
Class II transposable elements (TEs) that move in the host genome via a "cut and paste" mechanism are the most useful for genetic analyses, because of their easy laboratory handling and controllable nature. A schematic outline of the transposition process of a Tc1/mariner TE is presented in Figure 1a. Class II TEs are simply organized; they encode a transposase protein in their simple genome flanked by the inverted terminal repeats (ITRs). The ITRs carry the transposase binding sites that are necessary for transposition (Figure 1a). The transpositional process can easily be controlled by separating the transposase source from the transposable DNA harboring the ITRs, thereby creating a non-autonomous TE. In such a two component system, the transposon can only move by trans supplementing the transposase protein (Figure 1a,b). Practically any sequence of interest can be positioned between the ITR elements, depending on experimental need. Transposition will result in excision of the element from the vector DNA and subsequent integration into a new sequence environment.
In this review we discuss the utility of class II TEs for various genetic modifications in metazoan model systems. We do not cover applications of class I retrotransposable elements, such as L1; for coverage of such elements, the reader is referred to another review included in this supplement . We describe those features of the transposons that are important to consider for their proper use as genetic tools. Next, we provide an overview of their applications in the most prominent animal models, with a focus on Caenorhabditis elegans and Drosophila. Finally, we discuss and suggest directions for further development of transposon technology in vertebrate genetics.
General considerations in the application of transposons as DNA delivery tools
The class II TEs most frequently used in metazoan models are listed in Table 1. Five out of the eight TEs listed belong to the Tc1/mariner family. The predominant application of the Tc1/mariner elements results mainly from their broad host range  as compared with other TEs (for example, the P element is only active in Drosophila flies). The basic requirements for applicability of a TE in any given model organism are that there is a sufficient level of transpositional activity in the given host and that there is a lack of endogenous copies in the targeted host genome (in order to avoid mobilization of resident copies). Studies aimed at developing hyperactive transposon mutants have established that it is possible to increase transpositional activity using various laboratory modifications [3–5]. However, host restrictions of P elements could not be circumvented, despite much effort . Because host specificity barriers cannot easily be challenged, transposon based genetic technologies in all of the major model organisms were dependent on the discovery of TEs that are active in the species of interest (for details, see below). The use of TEs that originated from distantly related species could guarantee satisfaction of the second requirement, if they still exhibit acceptable activity in the desired host. However, cross-mobilization is not fully predictable and can be an issue, as was shown for the related hAT superfamily elements Hobo and Hermes .
Other important phenomena should also be considered when designing an individual experiment, such as cargo capacity of the TE, sensitivity to over-production inhibition (OPI), integration site preference, and transposition to linked chromosomal sites ('local hopping').
Capacity for cargo
For mutagenesis purposes, small TE vectors can be designed that retain two basic functions: the cis requirements for transposition and a mutagenic feature designed to disrupt normal gene function. However, size does matter for transgenesis purposes, including the generation of germline modified laboratory stocks of model species and species of biotechnologic interest, as well as for human gene therapy applications. In these instances, transgene constructs that include coding regions of genes with all of the necessary transcriptional regulatory elements can exceed several kilobases in size. The effects of increasing the size of the DNA fragments cloned between the ITRs of the different TEs are listed in Table 1. Tolerance for cargo size varies greatly between elements. Although a 100 kilobase extended P element that is capable of transposition has been reported , members of the Tc1/mariner family are inhibited by increasing size. The minimal 5' and 3' terminal sequences necessary for highly active transposition are also well defined for the elements listed in Table 1.
OPI describes a phenomenon of decreasing efficiency of transposition beyond a certain level of cellular transposase concentration. OPI has been described for a wide variety of TEs. Of the TEs listed in Table 1, it appears to affect at least the Tc1/mariner elements [3, 9] and piggyBac  (although a recent study  was unable to confirm OPI of piggyBac). Several lines of direct and indirect evidence suggest that Tc1/mariner transposases act as oligomers. OPI is thought to occur when transposase monomers are present in excess concentrations; thus, in the absence of available DNA substrate, they form inactive or weakly active oligomers. Therefore, increasing the amount of transposase protein can have an inhibitory effect on transposition and, accordingly, the ideal level of transposase expression is not necessarily the highest level. In case OPI is an issue in a given experimental setup, it is advisable to test several conditions for transposase expression.
Integration site preference
Target site preference varies among transposons. For example, at the level of primary DNA sequence, the Tol2 element does not appear to exhibit a pronounced preference for any sequence for insertion. In contrast, the piggyBac transposon targets the sequence TTAA, whereas all Tc1/mariner TEs target their integration into TA dinucleotides (Table 1). In the case of Sleeping Beauty (SB), this preference was studied in detail, and palindromic AT repeats were found to be preferred sites for integration . Computational analyses revealed that target selection is determined primarily on the level of DNA structure, and not by specific base pair interactions. It was shown that preferred target sites have a bendable structure and increased distance between the central base pairs [12, 13]. It is possible that similar structures are favored by other Tc1/mariner TEs. This could be interpreted as meaning that integrations will occur into any DNA available, depending solely on these preferences. This, however, is not the case. In the context of chromatin, Tc1/mariner elements have no or weak preference for transcription units, the 5' regulatory regions are disfavored, and most hits in genes are localized in introns (Table 1). On the contrary, the P element has a clear preference for the 5' regulatory regions of genes. The P element in this respect is similar to retroviruses, because murinie leukaemia virus prefers the 5' end of transcription units, whereas HIV exhibits strong preference for the entire length of transcription units (for review ). This control of integration at the chromatin level is poorly understood. One possible explanation for this can be the affinity of the transposase for unknown, chromatin associated factors. Supporting this hypothesis, a recent study showed that a host protein, lens epithelium derived growth factor, is involved in directing HIV integration into active genes . Integration site preference can greatly influence the utility of transposon vectors for different applications. For example, human gene therapy protocols would require application of transposon vectors showing the least preference for genes, for obvious safety reasons. On the contrary, mutagenesis screens can capitalize on elements that exhibit a tendency to land in genes. In this respect, the utility of transposons for mutagenesis is greatly enhanced by the availability of multiple vector systems with distinct preferences for insertion.
'Local hopping' describes a phenomenon of chromosomal transposition in which transposons have a preference to land into cis linked sites in the vicinity of the donor locus. Local hopping appears to be a shared feature of cut and paste transposons. However, the actual extent of hopping to linked chromosomal sites and the interval of local transposition varies. For example, the P element prefers to insert within about 100 kilobases of the donor site at a rate that is about 50-fold higher than that in regions outside that interval . Similarly, in germline mutagenesis screens in mice using SB, 30% to 80% of transposons have been observed to reinsert locally on either side of the transposon donor locus [17–19]. In contrast to the P element, SB appears to have a much larger local transposition interval between 5 and 15 megabases .
The local hopping feature not only differs between different transposons; a given transposon may also exhibit great variation in different hosts, and variations can be seen between different donor loci even in the same host. For example, in case of Ac element transposition in maize, about 50% to 60% of the reinserted elements were distributed within a 5 cM distance of the donor site [20, 21], whereas the frequency of local hopping greatly varies in Arabidopsis and tobacco, depending on the chromosomal location of the donor site [22–24]. Moreover, local hopping of the Ac element in tomato appears to be overall less prevalent than in maize [25, 26], and differences with regard to its tendency toward local hopping out of different transposon donor loci have been observed . This variation in local hopping of the same element could possibly be explained by varying affinity of the transposase to unknown, chromatin associated factors in different hosts . If that is the case, then it can be assumed that transposase mutants with altered tendency for local hopping could be created.
Local hopping can play a significant role in mutagenesis using chromosomally resident transposons. In practical terms, local hopping limits the chromosomal regions accessible to a transposon jumping out of a given chromosomal site. To circumvent this limitation, establishing numerous 'launch pads' to initiate transposition out of different loci can be a viable strategy to increase coverage of gene mutations. On the other hand, local hopping can be useful for saturation mutagenesis within limited chromosomal regions. Even for that purpose, however, starting with more donor sites could be the most effective arrangement, because even two donor sites in closely related loci can produce strikingly different local hopping frequencies .
Current state of applications of transposon systems in prominent metazoan model organisms
In all model organisms described in the following sections, the TEs are used via slightly different approaches to reach similar goals. This is because of the distinct biology of the model organisms. Alterations in culturing or maintenance and other features of the organisms, and the features of the TEs alike, all influence the methodology of harnessing transposons as experimental tools in the particular model systems.
Nematodes: Caenorhabditis elegans
In C. elegans, Tc1 and Tc3 (see Table 1) have been widely used for insertional mutagenesis during the past 20 years. The reason for this extensive use is their early discovery in this model organism. However, their use is also limited here because of two major drawbacks. First, all known isolates of C. elegans contain multiple copies of Tc1 and Tc3, which makes identification of the relevant mutagenic insertions difficult. The second drawback is that germline mobilization of Tc transposons cannot be controlled in mutator strains, in which these elements are active in the germline. However, these drawbacks can to some extent be circumvented, because the Tc insertion sites are well known in most of the laboratory strains, and because of differential transpositional activity in the germline of the different strains.
With respect to Tc1 copy numbers, the strains can be divided to low copy strains such as Bristol N2 (containing approximately 30 copies) and high copy strains such as Bergerac (containing >500 copies per haploid genome) [29–31]. Tc1 is active in somatic cells in all genetic backgrounds examined, but its germline activity is undetectable in Bristol and 1,000-fold lower as compared with somatic cells in Bergerac. Mutants have been isolated that exhibit increased Tc1 (and occasionally other TE) activity in the germline, and their certain derivatives have low Tc1 copy numbers. These mutant strains with elevated germline transposition rates are the so-called mutator strains. Generally, the mutations in the mutators affect the RNA interference and transgene co-suppression pathways . The mut-2 mutator exhibits the highest frequency of transposition, at about 40-fold above Bergerac . Some of its derivatives, in which the original mut-2 strain is back-crossed into the Bristol background, harbor fewer Tc1 copies. Intensive germline transposition in the mutator strains as well as stabilization of the new insertions by repeated back-crosses to low copy nonmutator strains can be achieved. The C. elegans model has significant advantages in supporting rapid crossing and selection procedures needed for mutagenesis by transposons.
More recently, use of the heterologous transposon Mos1 (Table 1) has also been established in C. elegans [34, 35]. The Mos1 elements are absent from the C. elegans genome; therefore, different experimental strategies involving this transposon could also be developed in C. elegans (see below).
Transposon-mediated reverse genetic approaches
Transformation of C. elegans is traditionally carried out by microinjection of DNA into the cytoplasm of the syncytial part of the gonad . This predominantly results in formation of long, extrachromosomal arrays (a special characteristic of C. elegans) that can pass through the germline. Infrequently, chromosomal integrations can also occur, depending on the injection conditions. Because this method is efficient, and the extrachromosomal arrays can be maintained in the transgenic strains for a long period of time, the transposon systems have not typically been utilized for the purpose of simple transgenesis.
Reverse genetics in C. elegans has been hampered by the practical inability to target specific mutations to a selected gene via homologous recombination based gene targeting. Developing this technology in C. elegans has been unsuccessful for a long time, because of the inefficient homologous recombination and chromosomal transformation in this model organism. Recently, these difficulties were addressed by the introduction of DNA into the worms using novel methodology, which involved more efficient harvesting of chromosomal integrations and use of the new selection marker unc-119 . This method is not yet in routine use, however.
TE based mutagenesis is suitable for the purpose of target selected gene modifications in C. elegans. This approach relies on screening mutant libraries created by transposon insertions. In C. elegans it is relatively easy to isolate a specific transposon insertion in any genomic region of interest, using a polymerase chain reaction (PCR) based sib-selection method . One difficulty in generating loss of function phenotypes with transposon insertions is that by using endogenous, unmodified Tc1-like elements, the chance for insertions creating null alleles is very low. For example, it was shown that animals homozygous for transposon insertions in the myosin light chain 2 (mlc-2) gene are phenotypically wild type. Interestingly, not even insertions in exons caused loss of function effects, because different atypical splicing events removed the Tc1 part out of the mlc-2 pre-mRNA, leaving only small, in-frame deletions and insertions . Analysis of five more Tc1 insertions in two other genes revealed that each mutant expressed substantial quantities of mature mRNA from which most or all of the Tc1 sequences have been removed.
To circumvent the above problem and to obtain knockouts via TE insertions, a strategy of searching for chromosomal deletions following TE excision can be used. The following mechanism is suggested to explain transposition associated deletions. TEs generally create target site duplications upon insertion and leave footprints upon excision. These footprints are generated when the double strand break (DSB), created by the transposase at the excision site, is repaired by the nonhomologous end joining DNA repair pathway (Figure 1b). Alternatively, the DSB can undergo homology dependent DNA repair (HDR). This may not result in any change to the original sequence, if the wild-type homologous chromosome is available as template, and it is used for the repair. HDR can also fill back transposon sequences to different extents, in case a homologous template containing the transposon is available for repair (Figure 1b). However, one of the free DNA ends can scan the DNA at the other end for a short homology; when this is encountered, DNA repair reactions ligate the two ends, thereby deleting the intervening DNA. In the study conducted by Zwaal and coworkers , gene specific PCR primer pairs were used to detect Tc1 insertions in five genes, and subsequently to detect the DNA repair mediated partial deletions of these genes following transposon excision. Such deletion derivatives were detected at a surprisingly high frequency (>10-3). This approach is definitely useful in a model organism such as C. elegans that has short generation time and easy culturing properties.
However, the transposon insertion-deletion method described above has limitations as compared with homologous recombination based approaches. Namely, it is limited to isolating only those deletions that are of a size that is detectable by PCR and that occur between the two predetermined gene specific primers; therefore, it is not useful for creating gene mutations other than null alleles. To circumvent these limitations, a method based on transgene directed, transposon mediated gene conversion was recently introduced . This approach capitalizes on the observation that an episomal transgene construct can also serve as a template for the repair after the excision of the TE. In this protocol, a plasmid carrying an engineered gene modification and some regions homologous to the targeted locus is introduced into a mutator C. elegans strain harboring the gene specific Tc1 insertion. This strain is then expanded into independent populations, in some of which the DSBs generated by transposon excision are repaired from this extrachromosomal template. These populations are subsequently tested for the presence of the desired mutation. The efficiency of this method seems to be about tenfold higher than that of the standard insertion-deletion approach mentioned above. Recently, the protocol was adapted to the use of Mos1 transposition in worms . The advantage of using a heterologous TE is that background transposition events can practically be ruled out.
Transposon mediated forward genetic approaches
Mutagenic insertions for forward genetics involve molecular tags that are used to clone the mutated gene rapidly. Therefore, the above strategy utilizing the Tc1 transposon is rather cumbersome for use in forward genetics research in C. elegans, because the Tc1 insertions do not provide unique tags, and so it is difficult to identify the relevant insertion responsible for a given phenotypic change. Moreover, the Tc1 elements are active in all C. elegans strains, at least in their soma. Therefore, a phenotype driven insertional mutagenesis screen is more promising by using the heterologous transposon Mos1, which expedites the process of identifying the mutated genes [35, 43]. It has been shown that mobilization of Mos1 can also be carried out via the generally used binary system of a non-autonomous transposon and a separate transposase source (Figure 1a). These two components are maintained as extrachromosomal arrays in separate strains, and expression of the transposase protein is controlled by a heat shock promoter . The mutagenicity of the Mos1 system is in the range of that of Tc elements in mutator strains . Therefore, the newly developed Mos1 system is a promising tool for use in insertional mutagenesis in C. elegans.
Insects: Drosophila melanogaster
The predominantly used transposable elements in Drosophila are the P element, piggyBac, Mos1, and Minos (Table 1). The two closely related hAT elements Hobo and Hermes are also used to some extent, essentially for simple transgenic purposes. The most prominently used transposon in Drosophila has been the P element. P elements are currently active resident TEs in Drosophila. They have a very narrow host spectrum, because they are not active outside the Drosophila genus. P elements are thought to be very recent invaders of the D. melanogaster genome, because they were present in recently wild caught strains but not in laboratory stocks established during the first half of the past century. The source of this horizontal transfer was presumably another Drosophila sp. The early discovery of the P element, its high transpositional activity, and the P-element-free nature of the D. melanogaster laboratory strains have made this transposable element the workhorse of Drosophila genetics research. Early mutagenesis schemes, similar to some extent to the C. elegans mutator strain system, were based on crossing two strains to mobilize P elements in the genome, exploiting the phenomenon of P-M hybrid dysgenesis [44, 45]. However, use of hybrid dysgenesis was soon exchanged for the easily controllable binary system mentioned earlier. In contrast to Tc1 in C. elegans, building of this system in Drosophila was facilitated by the fact that the P element has no resident copies in the D. melanogaster laboratory strains. This allowed the generation of transgenic stocks each containing a separate component of the binary transposon system in its genome: one element, encoding the P element transposase, is carried by the 'jump starter' strain, which, upon inter-crossing, efficiently mobilizes the second, non-autonomous transposon in the genome of the 'mutator' strain . This system is extremely suitable for forward genetics applications.
Genetic transformation in Drosophila is traditionally done by the injection of preblastoderm embryos . Enhancement of this transformation procedure via TE transposition into the genome is a widespread technique. Practically, all TEs listed above are successfully used for this purpose in Drosophila. The injection of in vitro synthesized mRNA as a transposase source can further enhance the efficiency of this technique because of the more rapid availability of the transposase, resulting in reduced transgene mosaicism in the embryo and therefore elevated germline transmission rates. For example, in the case of Minos based transformations, such methods have been shown to yield germline transgenesis rates about tenfold higher as compared with straight plasmid injections . Moreover, the application of insulator sequences in combination with TEs can facilitate reliable transgene expression, and may protect endogenous genes from the effect of enhancer elements carried by the transposon construct. Indeed, a recent study demonstrated the usefulness of scs/scs', gypsy, and β-globin HS4 insulators to minimize position effects influencing the expression of transgenes delivered by the piggyBac transposon in Drosophila .
Transposon-mediated reverse genetic approaches
Homologous recombination is fairly inefficient in flies. Thus, classical gene targeting, as applied in mouse embryonic stem (ES) cells, has not been successfully established in Drosophila. However, induced DSBs can enhance recombination to some extent, and can trigger HDR at the breakpoints; therefore, the excision of TEs can efficiently facilitate gene conversion events. Utilizing this phenomenon, targeted gene replacement in Drosophila via P element induced gap repair has already been reported (some 15 years ago) . P elements have also been used for the isolation of rare deletion derivatives after element excision from a gene of interest, to obtain null alleles , long before such a strategy was applied in C. elegans.
Transposon-mediated forward genetic approaches
Insertional mutagenesis using engineered TEs has proven to be one of the most productive and versatile approaches to disrupting and manipulating Drosophila genes on a genome-wide scale, and by far it leads the field among metazoan model systems. The experimental strategies generally utilize the 'jump starter/mutator' experimental setup, as described above. The usefulness of these screens is strongly promoted by the highly developed classical genetic tools and methods in Drosophila.
The P element has been the most widely used vehicle for these purposes. The mutagenicity of P element insertions is higher than that of Tc1/mariner elements (Table 1). Moreover, P elements appear to transpose efficiently with large cargo sequences inserted within the transposon (Table 1). The early mutagenesis screens carried out in Drosophila utilized vectors that harbor marker genes that are easy to screen such as white, and functional bacterial components (antibiotic resistance genes, origins of replication) that aid molecular analysis of the transposon insertion sites. Vectors of later generations were equipped with gene trapping features, representing an improvement to the basic design. The basic strategies employed to enhance the mutagenicity as well as reporting capabilities of insertional vectors by trapping transcription units are shown in Figure 2. Moreover, elements of binary systems for controlled gene expression such as the GAL4 DNA binding transcription factor (GAL4)/GAL4-upstream activator sequence (UAS) system, or for site-directed recombination such as the flip recombinase (FLP)/FLP recombinase target (FRT) system have also been incorporated into advanced vectors. Thus, a range of versatile experimental designs using P elements for insertional mutagenesis has been developed.
Enhancer trap screens are designed for the identification of enhancers by activating a reporter gene within the P element (Figure 2b). In early enhancer trap versions, the transposase promoter itself was utilized as a weak promoter to capture the enhancers in the genome . Gene trapping is based on the activation of a promoterless reporter gene that is dependent on splicing between the exons of the trapped gene and a splice acceptor site carried by the transposon (Figure 2c). Thus, gene trap vectors both report the insertion of the transposon into an expressed gene, and have a mutagenic effect by truncating the transcript through imposed splicing.
Both enhancer and gene trap vectors have been combined with the yeast GAL4/UAS transcription activation system (Figure 2). For example, enhancer detection vectors that direct the expression of GAL4 in a genomic integration site dependent manner have been developed . Therefore, such vectors report the expression pattern of trapped enhancer elements, and can also activate a cloned, UAS driven gene of interest in a tissue specific manner (specifically, in those cells in which GAL4 is expressed). The system proved to be highly useful for identifying genes that are involved in a variety of biological processes, and many GAL4 driver lines have been created and made available to the research community .
More sophisticated vectors that contain a polyA trap cassette that reports insertion into a Pol II transcription unit have also been developed (Figure 2d). Because polyA trap cassettes have their own promoters, they can report insertion into genes irrespective of their expression status in a given cell type. Importantly, polyA trapping is not expected to be mutagenic, because the vector is not designed to express the downstream exons of the targeted gene at the protein level. Therefore, polyA trap insertions are unlikely to cause dominant effects. Dual tagging systems that combine both gene trap and polyA trap elements (Figure 2e) have been used both in mouse  and in Drosophila .
Protein trapping (Figure 2f), similar to the trapping systems described above, is also based on hybrid splicing events between an endogenous gene and the transgene cassette carried by the transposon; however, the vector is designed to ensure that the inserted reporter manifests at the protein level. A protein trap strategy to detect GFP tagged proteins expressed from their endogenous loci has been developed by Morin and coworkers . The P element based PTT vector was constructed to tag proteins randomly with an enhanced GFP, without disrupting their subcellular localization. PTT carries an artificial exon that encodes GFP and is deprived of initiation and stop codons but flanked by splice acceptor and donor sequences. To enhance protein tagging efficiency, a series of constructs were created to allow reporter gene activation in each of the three reading frames (Figure 2). GFP chimeras typically retain the localization properties of the trapped proteins, except when GFP disrupts a domain necessary for subcellular targeting. Thus, transgenic lines exhibiting tissue specific GFP expression and targeting the GFP signal to virtually any compartment of the cell can be recovered. A disadvantage of the system is that it relies on the relatively rare intronic insertions of the P element. Other transposons such as piggyBac may produce more intronic insertions, which may be better suited to the requirements of such a screen (Table 1; also see below).
Another way to manipulate a trapped transcription unit that has already been proven to be useful is the targeted over-expression and/or mis-expression system (Figure 2g). Using this method, one can bring about over-expression of the full length or truncated protein product (depending on the position of transposon insertion) of the targeted gene, thereby producing dominant phenotypes by overdosing the affected gene product. An improved version of this method is the modular mis-expression system developed by Rorth . It allows directed mis-expression of P element targeted genes in any temporal or spatial pattern. It is practically the reversal of the GAL4/UAS system. This modular mis-expression system benefits from the insertional preference of P element; specifically, it tends to insert upstream of the ATG codon of transcription units . Therefore, the integrated transposon carrying UAS enhancer and promoter elements can frequently over-express the native full length protein. Such insertion screens can identify genes that, when over-expressed or mis-expressed in a pattern of interest, give a specific phenotype or modulate an existing mutant phenotype. For example, in the first screen conducted by Rorth , when activated in the developing eye, 4% of insertions gave a dominant phenotype. The next study by Rorth and coworkers  demonstrated the usefulness of the system in genetic interaction screens. They identified many known and new genes involved in the migration of border cells in the ovary, by suppressing the cell migration defect on a mutant background.
An important consideration for the mutagenicity of any transposon is its insertional preferences. The insertion pattern of P elements (and that of all other TEs) is non-random (Table 1). Moreover, P element insertions have numerous 'hotspots' and 'cold regions' on a genome wide scale. Investigators at the Berkeley Drosophila Genome Project have created and analyzed large collections of insertions utilizing some of the vectors mentioned above . They found that, interestingly, the observed hotspots can be divided to 'common hotspots' and 'screen specific hotspots'. The first class is commonly hit by all P element vectors, whereas the second is preferentially hit only in a particular mutator strain . Hotspots seen in local hopping are excluded from the second class. The existence of screen specific hotspots suggests that the specific parameters of the screen, such as the structure and location of the mutator transposon, can affect the spectrum of hotspots and the diversity of the targeted genes. This phenomenon is poorly characterized, and the underlying cellular mechanisms remain unclear.
Common hotspots represent the main obstacle to full genome coverage with P element vectors. It is estimated that about 150,000 P element insertions might need to be screened to obtain 87% saturation of the estimated 13,500 Drosophila genes . To complement the use of P elements, alternative transposon systems have successfully been contributing to large scale insertional mutagenesis of the Drosophila genome. For example, investigators at the Berkeley Drosophila Genome Project have already included piggyBac and Minos element based screens in the collection. A large scale comparison of the insertion patterns of piggyBac and P element vectors has already been reported . It has been found that piggyBac exhibits an insertional preference that is distinct from that of P elements. It does not share chromosomal hotspots that are associated with P elements and, although piggyBac favors genes as targets, it lacks the bias for 5' regulatory sequences . The target preference of Minos also differs from both P elements and piggyBac, and appears to be similar to that of SB (Table 1). Therefore, these TEs are used as complementary tools for Drosophila mutagenesis.
The combined use of different TEs is common in Drosophila. Practically all of the insertional mutagenesis screens have been established by the creation of 'jump starter' and 'mutator' P element lines, whose generation is facilitated by use of other TEs, generally the Hobo or Hermes elements. For some more sophisticated screening strategies, it is also important to have alternative TEs for effective insertional mutagenesis on a background already carrying P elements and possibly also Hobo or Hermes. Hacker and coworkers  used piggyBac for insertional mutagenesis on a chromosome harboring P element inserted FRT sites for the generation of mitotic recombinants. The FRT sites remained stably integrated, demonstrating that the two systems are compatible.
Chromosomal deletions in Drosophila are indispensable, classic genetic tools for mapping mutations, characterizing alleles, and identifying interacting loci. The P element based methods for creating deletions are extremely useful because the end-points of the deletions are molecularly marked. Furthermore, their positions can be designed, which is of particular importance in avoiding haplolethal or haplosterile loci. Two P element based methods are in predominant use to create chromosomal deletions . One is based on the observation that P transposase often induces chromosomal aberrations that involve the sites of two distinct P element insertions. The process behind this is called 'hybrid element transposition', in which the TE ends come from separate elements rather than a single element (the 5' end of one element pairs with the 3' end of another one at a different location) . This results in different chromosomal rearrangements from which the deletions can be selected. An improved version of the transposon based method for creating deletions makes use of the FLP/FRT site specific recombination system (Figure 3a). Transposon vectors, usually the P element, are used to facilitate single copy chromosomal integration of FRT sites. FLP mediated recombination between two of these P elements can result in chromosomal rearrangements. With a sufficiently high density of starting insertions, even single gene deletions can be created. Progress is currently being made toward covering the genome of Drosophila with characterized deletions .
This technique can also create predesigned chromosomal translocations between the chromatids in flies with transgenic FRT sites at identical positions on the homologous chromosomes . Thus, FLP mediated recombination can be used to generate mitotic clones (Figure 3b), in which only clones of the cells of interest are homozygous for the studied mutation, whereas the rest of the organism is heterozygous. Spatially or temporally controlled expression of FLP recombinase can create homozygous clones in any tissue or developmental stage of interest.
Chromosomal inversions are also powerful tools in classical Drosophila genetics. They have been applied in the majority of genetic screens in Drosophila as balancer chromosomes, because they can block recombination within the region of the inversion. For practical reasons, the balancers carry visible markers, and are also designed to be recessive lethal. Most of them were isolated as spontaneous or induced chromosomal rearrangements having break points in vital genes. TEs have not been typically used to engineer balancers. The balancers greatly help to map and maintain mutations in the Drosophila genome.
Transposons have successfully been used in lower metazoan and plants for transgenesis and insertional mutagenesis, but until the reactivation of the SB transposon system in 1997  there was no indication that any DNA based transposons in vertebrates were sufficiently active for these purposes. Subsequently, other elements were shown to catalyze efficient transposition in vertebrate model organisms. For example, the insect TEs piggyBac and Minos have proven to be useful in germline mutagenesis in vertebrates [68, 69]. Moreover, the reconstructed endogenous amphibian element Frog Prince , the reconstructed human Hsmar1 element , and the Tol2 element isolated from the medaka fish  have been found to be active in vertebrates. We do not extensively review current transposon applications in vertebrate models here (other reviews in this supplement provide coverage of these areas). However, we do discuss the general approaches that have been taken, and suggest further avenues for exploiting TEs in applications in vertebrates.
Transposon based experimental strategies in vertebrates all utilize the two component, binary approach, in which transposition is controlled by trans supplementation of the transposase proteins, owing to the fact that the majority of these TEs are not endogenous in the most important model organisms.
Classic ways to induce expression of foreign genes in vertebrates rely on microinjection of nucleic acids into oocytes or fertilized eggs. Two main drawbacks of these approaches are the low rates of genomic integration and that the injected DNA generally integrates as a concatemer. Both drawbacks can be circumvented by utilizing transposition mediated gene delivery, because it can increase the efficiency of chromosomal integration and facilitates single copy insertion events. Single units of expression cassettes are presumably less prone to transgene silencing than are the concatemeric insertions created using classical methods. Retroviral vectors are also useful tools for the same purpose, but their integration pattern is potentially more mutagenic because of their preference for the 5' end of transcription units (for review ). In case of transgenesis, a single copy insertion away from endogenous genes is clearly desired. The insertional spectrum of Tc1/mariner elements satisfies this need the best (Table 1), because these elements integrate randomly at the genome level, and do not exhibit pronounced bias for integration into genes. Another particular problem concerning transgenesis is that founders that develop from the injected oocytes or eggs are predominantly mosaic for the transgene, because integration generally occurs relatively late during embryonic development. Therefore, in order to promote successful transmission of the transgene through the germline to the next generation, it is necessary to shift the window of integration events to as early as possible. This can be facilitated by co-injection of engineered transposons with transposase mRNA. This method has been employed to generate transgenic zebrafish with Tc3 , Mos1 , Tol2  and SB ; transgenic Xenopus with SB  and Tol2 ; and transgenic mice with SB [78–80].
Transposon mediated forward genetic approaches
To carry out phenotype-driven forward genetic screens in vertebrates, one must achieve efficient germline mutagenesis. To date, the most efficient mutagen in the mouse germline is the chemical N-ethyl-N-nitrosourea (ENU). Mutagenesis rates using ENU are two to three orders of magnitude higher than those with insertional mutagens . However, ENU is an ethylating agent that generally causes single base pair mutations. Therefore, the average phenotypic effect of an insertional vector can be more dramatic, and the total number of insertions required to reach the same mutagenic effect is expected to be lower. Moreover, identification of the point mutations causing a phenotype requires positional cloning, which is time consuming and laborious work. Therefore, insertional mutagenesis is an attractive alternative to ENU screens.
Both TEs and retroviral vectors can successfully be applied to insertional mutagenesis. Cultured cells can be efficiently infected with viruses . A pseudotyped retrovirus has also been applied to generate insertions in zebrafish via microinjection of virus particles into blastula stage embryos . In this approach, however, the transgenic founder fish aremosaic and must be out-crossed to establish F1 fish with retrovirus insertions. Therefore, one drawback of the application of retroviruses is that the convenient 'jump starter' and 'mutator' method is not applicable with these vectors. Moreover, handling of such viruses may bring up safety issues.
Using TEs as tools for insertional mutagenesis is simpler, and the 'jump starter' and 'mutator' scheme can be applied. In Drosophila, transposon mediated insertional mutagenesis is predominantly carried out using such a scheme. This is also the preferred method in vertebrates, and it has successfully been adopted for germline mutagenesis in the mouse, but not in zebrafish, in which the screens are currently performed by co-injection of the transposon DNA and the transposase mRNA.
In zebrafish, SB and Tol2 were shown to be useful for insertional mutagenesis in co-injection experiments [84–88]. In the mouse, it has been demonstrated that SB, Minos, and piggyBac transposases can function in transgenic animals [17, 18, 68, 78, 89–92]. Recently, SB based insertional mutagenesis was also established in the rat [93, 94]. In these experiments, chromosomally resident transposon vectors were mobilized in transgenic animals that either ubiquitously expressed the transposase or expressed the transposase in the male germline using the protamine 1 (Prm1) promoter. SB based insertional mutagenesis has successfully been applied in mice to recover a range of mutant phenotypes in a crossing scheme applying a balancer chromosome . This and other studies  demonstrated that local saturation mutagenesis of a genomic region is a realistic goal using the SB transposon system with a chromosomally resident transposon donor site. The Minos transposase has also been shown to mobilize non-autonomous Minos elements in mice by transposase expression in the oocytes using ZP3  and in the lymphocytes using CD2 promoters . PiggyBac has also been used in co-injection experiments in mice . The activity of Tol2 element has already been demonstrated in mouse ES cells  and in vivo in the mouse liver .
All of the vectors used in vertebrate insertional mutagenesis to date are versions of gene trapping insertional mutagenic constructs (Figure 2), equipped with elevated mutagenicity and other useful properties. The mutagenicity of gene trap vectors is higher than that of simple insertional vectors, and they enable easy identification of the mutagenized gene by reverse transcription PCR of composite transcripts composed of sequences of the insertional vector and the endogenous gene. In cell culture, drug resistance markers are generally in use, whereas in animal systems other reporters such as GFP are sufficient for this purpose. Similar to the GAL4/UAS system in Drosophila, a conditional, tetracycline regulated system has been shown to be applicable to TE mediated insertional mutagenesis in mice .
As an alternative to the loss of function approaches, targeted over-expression and/or mis-expression has been shown to be efficient in somatic tissues of mice using SB. Viral enhancer promoter elements incorporated into SB vectors were shown to be useful in inducing cancer in experimental animals [100, 101]. These screens can also capitalize on TEs with an intronic preference for insertion, such as members of the Tc1 family. In order to devise customized screens for cancer development, a current approach is focusing on establishing mouse lines that conditionally express the transposase . One approach is to express the transposase from tissue specific promoters. The second is to generate a Cre recombinase inducible transposase allele, and to take advantage of the many existing Cre strains to induce mutagenesis in specific tissues in mice .
The parallel development and application of alternative transposon systems will be beneficial for insertional mutagenesis in vertebrates. As described above, P elements, piggyBac, and Minos elements are already in use as complementary transposon tools for large scale mutagenesis in Drosophila [60, 62]. The combined use of these TE systems makes full genome coverage with TE based insertional mutagenesis a realistic goal. Work to create comprehensive mutant collections is already underway in mice by the Knockout Mouse Project (National Institutes of Health, US) and by the European Conditional Mouse Mutagenesis project. The goal of these initiatives is to knock out every single gene in mouse ES cells using conditional gene trapping and gene targeting approaches. It is therefore likely that collections of transposon insertional mutants for reverse genetic purposes will prove even more useful in species that lack efficient homologous recombination based gene targeting techniques and ES cells, such as zebrafish, Xenopus tropicalis, and rats.
The 'jump starter' and 'mutator' experimental scheme is widely used in both Drosophila and mice. Even though microinjection does not appear to be a bottleneck in transposition based transgenesis in zebrafish, establishing a mutagenesis set-up based on breeding could be beneficial. With this method, the numerous injections of fertilized eggs could be eliminated, and transposition events segregated into offspring by simple crossing of founders. Moreover, local saturation mutagenesis would also be possible in this way in zebrafish. In mice, the existence of the mutator lines and the local hopping feature of the TE systems offers the possibility of using local saturation mutagenesis to screen through chromosomal regions harboring as yet unidentified genes in which disease causing mutations occur.
Insertional mutagenesis with SB in both germline and somatic tissues of the mouse has been approached with mutator lines harboring transposon donor loci containing many copies of the transposon vector in the form of concatemeric arrays. The reason for this is that transposition rates out of multicopy concatemers is far more efficient than out of single copy donor sites. Consequently, Dupuy and coworkers  used founder lines with 148, 214, and 358 transposon copies in concatemeric donor sites, whereas Collier and colleagues  worked with animals containing approximately 25 copies of the mutagenic transposon in somatic mutagenesis studies. Similarly, a concatemeric donor site of approximately 30 transposon copies was used in a gene trap germline screen in mice . However, transposition out of multicopy donor loci may complicate assignment of a phenotype to a particular transposon insertion in at least two ways. First, a phenotype may be associated with multiple insertion events, and segregation of the insertions may lead to loss or change in the phenotype. Second, recombination between newly transposed transposon copies and the donor concatemer could lead to unwanted genomic rearrangements, as was observed by Geurts and coworkers . The most likely explanation for the rearrangements is that transposition out of a concatemer generates new transposase binding sites linked in cis (in case of local hops) or on other chromosomes. However, because transposon copies remain at the original donor locus, transposase can recombine chromosomal sequences that are located between the transposase binding sites by hybrid element transposition (described in the section on Drosophila, above), leading to deletions and translocations. Alternatively, hybrid element transposition involving transposon copies in the donor concatemer could result in similar genomic rearrangements. Such chromosomal rearrangements are unlikely to occur (or would occur at a much reduced frequency) if a single copy donor was used. Thus, there is a great need for transposon systems that are sufficiently active for efficient transposition out of single copy donors in animal breeding schemes. Ongoing work in our laboratory aiming at the isolation of hyperactive transposases could potentially eliminate the need for concatemeric donor sites.
The use of single-copy donors would also enable the application of dosage-dependent color markers such as tyrosinase and agouti for phenotypic marking of transgenic animals. These markers could be exploited to confer a light brown or a much darker color to an albino coat, depending on whether they are present as single- or double-copy transgenes in the mouse genome, respectively. This would be helpful to identify homozygous transposon insertions.
The approach used for the creation of the PTT vectors (Figure 2) in Drosophila would possibly enhance the utility of protein over-expression studies in mice as well. In two somatic mutagenesis studies in mice, the trapped genes were over-expressed from a viral long terminal repeat carried by the SB transposon [100, 101]. In these experiments, transcription started from the viral enhancer promoter and the resulting pre-mRNA was spliced between a splice donor site carried by the transposon vector and the downstream exon of the trapped gene (Figure 2). However, translation of the hybrid mRNA (and generation of a sense protein product) is dependent on the fortuitous occurrence of an in-frame ATG codon in the downstream exons. This can clearly be a limitation to successful over-expression events. To circumvent this problem, we propose that, similar to the PTT vectors applied in Drosophila (Figure 2), splice donor sites set to phases 0, 1, and 2 (according to the three possible reading frames) and built in behind a strong mammalian translation initiation consensus sequence could be used in over-expression studies. Because the intron phase distribution of mouse genes is unequal , using only the phase 0 construct could result in a success rate of about 50% in terms of trapping potential.
In the over-expression experiments mentioned above, the transposase was continuously expressed in the soma. This could result in multiple rounds of transposition events of the same transposon copy. Therefore, for these and possibly other experimental set-ups, it would be beneficial to limit secondary jumps by transposon immobilization after transposition . One possibility in this regard would be to use recombinase systems, where FRT or loxP sites could be inserted within the ITRs. This way, Cre or Flp mediated recombination would result in the partial loss of the ITR and a part of the internal transposon sequences, and so the resulting defective transposon would not be able to move again. The caveat of this strategy is that insertion of FRT or loxP sites could negatively affect transposition of the modified element.
The most effective agent in terms of mutagenicity is the widely used chemical mutagen ENU. The application of ENU is an efficient method in mice, but the precise identification of the mutations in a screen requires a laborious positional cloning approach. Classical genetic tools similar to those extensively used in Drosophila could facilitate this identification process. In this respect, both nested deletion sets and balancers over different loci could be especially useful in mouse forward genetics screens. One particularly interesting transposon based experimental system for insertional mutagenesis and chromosomal rearrangements, developed by Osborne and coworkers in Arabidopsis , could facilitate the creation of these genetic tools. Briefly, in this arrangement, the advantages of Ac/Ds transposition and the Cre-lox system were combined in Arabidopsis. The Dslox transposon, carrying the phosphonothricin (Ppt) resistance gene and a loxP site just in front of a promoterless gentamicin resistance (Gn) gene, jumps out of a donor locus harboring the chlorsulfuron (Cs) resistance gene and another loxP site between a strong plant promoter and the Cs coding sequence (Figure 4a). The excision and reintegration of the Dslox transposon may result in double PptR and CsR phenotypes. Subsequent Cre mediated recombination leads to two types of chromosomal rearrangement; deletions are associated with GnR phenotype and clearance of PptR and CsR phenotypes (Figure 4b), whereas inversions are associated with a GnR phenotype and silencing of the Cs resistance gene (CsS; Figure 4c). The other important key features of the system are the single copy donor sites at different chromosomal positions that make herbicide selection for coupled excision and reinsertion possible, and the local hopping feature of Ac transposition that generates the dominantly useful arrangement of two loxP sites for inversions and deletions of intervening DNA of different length. The system results in inversions, deletions, and smaller numbers of translocations, creating different resistance palettes and different phenotypes and viability. This system can be used to map loci with nested deletions and to establish balancer chromosomes from the inversions .
In case of vertebrates, composite arrangements of transposons carrying a loxP site embedded in another TE that carries the other loxP site could facilitate the generation of allelic series of local hops out of single copy donor sites. The Tol2 and piggyBac systems, having larger cargo tolerance, appear to be suitable for the delivery of such a complex arrangement. Transposition of the inner element out of the donor locus would move one loxP away, whereas the other loxP would stay at the original site. This system, based on the subsequent Cre-mediated chromosomal engineering between the transposed loxP sites, would greatly facilitate the creation of both of the two experimental tools in mice described above: viable balancer chromosomes and chromosomes bearing large deletions for establishing segmental haploidy.
Balancer chromosomes usually contain one or more inverted segments, and they suppress recombination within those segments. They are used as genetic tools to maintain recessive lethal mutations, providing an easy selection system for the heterozygous carrier animals. Balancer chromosomes are extensively used in Drosophila and also proved to be very useful in mouse genetics [106, 107]. In Drosophila, because many animals are allowed to mate randomly, and several generations can be maintained in one tube, the balancer must contain a homozygous embryonic lethal mutation. These recessive lethal mutations are generally defined by the end-points of the inversion, in which a gene necessary for embryonic development is broken. In contrast, mice are maintained as single mating pairs, and the offspring can easily be selected and separated. This means that the recessive embryonic lethal mutation on the balancer chromosome could be replaced with a visible marker, allowing the discrimination of animals that are heterozygous or homozygous for that marker . This improvement permits discrimination of the embryonic lethal mutations generated in a screen from the mutation carried by the balancer, and it makes the creation of useful balancers without pre-defined end points possible. Such an improved mouse balancer chromosome has been reported by Nishijima and coworkers . They used two coat color markers, tyrosinase and K14-agouti, and therefore the dosage of the inversion chromosome could be visually recognized.
Because of their usefulness, a current goal of the mouse community is to establish balancers that cover the entire mouse genome. Technologies based on transposition could be developed to create a series of viable inversions bridging over a genomic locus using an experimental scheme similar to the one developed by Osborne and coworkers  in Arabidopsis. The donor chromosome is generally favored for insertion over the other chromosomes in SB transposition about 60% of the time, with about 40% occurring in a 5 to 15 Mbp local hopping window and about 20% outside the typical local hopping range, but still chromosomally linked to the donor locus [95, 96]. Thus, a large portion of transposition events could yield potentially useful chromosomal rearrangements in mice.
Chromosomes harboring segmental haploidy can be used for deletion mapping of loci. An effective approach for mapping novel recessive mutations is based on a nested chromosomal deletion set, in which the deletions vary in size and have different end-points, but they partially overlap across the locus suspected of carrying the candidate gene affected by the mutation. After crossing these mice with a mouse strain carrying a novel recessive mutation, the recessive phenotype is observed when the deletion spans over the mutated gene on the other allele, and therefore no wild-type gene product is present.
The classical gene targeting approach to create these deletions would require two targeting steps for each deletion end-point (for review ). It is a laborious work, especially in the case of nested deletion sets, despite the fact that one end-point could be common for all of the deletions. Moreover, it is difficult to predict the viability of a given chromosomal rearrangement. To circumvent these difficulties, a deletion set has been made where the second endpoints of the deletions were defined by a randomly integrating recombinant retrovirus that carried the second loxP site necessary for Cre mediated rearrangements . Recently, this method has been further developed by delivering both of the loxP sites into the genome of mouse ES cells via retroviral gene transfer . In this study, the authors created two recombinant retroviruses, one of which, referred to as 'anchor virus', introduced the first loxP site, whereas the other, referred to as 'saturating virus', introduced the second loxP site into the genome of ES cells. The drug selection system applied by these authors was fairly similar to the one used by Osborne and coworkers in Arabidopsis . Although these methods based on the application of replication-defective retroviruses proved to be useful, one can predict that a transposon-based system that exploits local hopping of transposons, and guarantees single-copy insertion of the second loxP site, would represent an efficient and elegant approach to the creation of nested chromosomal deletion sets in mice.
Significant progress has recently been made toward the development of improved transposon based systems for genome manipulations in vertebrate model organisms, including transgenesis and insertional mutagenesis in both germline and somatic tissues. These efforts begin to pay dividends to the research community, as we witness an increasing interest in applying transposon tools for applications ranging from simple tissue culture setups to generate transgenic cell clones to experimental systems aiming to unravel genetic networks cooperating in tumorigenesis using transposon mutagenesis in living animals. Nevertheless, applications of transposons for vertebrate genetics are still lagging somewhat behind the sophisticated, transposon-based technology platform that has been established in invertebrate model systems, especially in Drosophila. We highlighted in this article possible improvements, and new avenues for the use of transposons in vertebrates, based on the lessons that have been learned in invertebrates. This 'technology transfer' offers a possibility to expoit transposable elements as gene delivery agents to their full potential.
Ostertag EM, Madison BB, Kano H: Mutagenesis in rodents using the L1 retrotransposon. Genome Biol. 2007, 8 (Suppl 1): S16-
Plasterk RH, Izsvak Z, Ivics Z: Resident aliens: the Tc1/mariner superfamily of transposable elements. Trends Genet. 1999, 15: 326-332. 10.1016/S0168-9525(99)01777-1.
Zayed H, Izsvak Z, Walisko O, Ivics Z: Development of hyperactive sleeping beauty transposon vectors by mutational analysis. Mol Ther. 2004, 9: 292-304. 10.1016/j.ymthe.2003.11.024.
Baus J, Liu L, Heggestad AD, Sanz S, Fletcher BS: Hyperactive transposase mutants of the Sleeping Beauty transposon. Mol Ther. 2005, 12: 1148-1156. 10.1016/j.ymthe.2005.06.484.
Pledger DW, Coates CJ: Mutant Mos1 mariner transposons are hyperactive in Aedes aegypti. Insect Biochem Mol Biol. 2005, 35: 1199-1207. 10.1016/j.ibmb.2005.06.002.
O'Brochta DA, Handler AM: Mobility of P elements in drosophilids and nondrosophilids. Proc Natl Acad Sci USA. 1988, 85: 6052-6056. 10.1073/pnas.85.16.6052.
Sundararajan P, Atkinson PW, O'Brochta DA: Transposable element interactions in insects: crossmobilization of hobo and Hermes. Insect Mol Biol. 1999, 8: 359-368. 10.1046/j.1365-2583.1999.83128.x.
Ring BC, Bass HW, Garza D: Construction and transposition of a 100-kilobase extended P element in Drosophila. Genome Res. 2000, 10: 1605-1616. 10.1101/gr.151700.
Lohe AR, Hartl DL: Autoregulation of mariner transposase activity by overproduction and dominant-negative complementation. Mol Biol Evol. 1996, 13: 549-555.
Wu SC, Meir YJ, Coates CJ, Handler AM, Pelczar P, Moisyadi S, Kaminski JM: piggyBac is a flexible and highly active transposon as compared to Sleeping Beauty, Tol2, and Mos1 in mammalian cells. Proc Natl Acad Sci USA. 2006, 103: 15008-15013. 10.1073/pnas.0606979103.
Wilson MH, Coates CJ, George AL: PiggyBac transposon-mediated gene transfer in human cells. Mol Ther. 2007, 15: 139-145. 10.1038/sj.mt.6300028.
Vigdal TJ, Kaufman CD, Izsvak Z, Voytas DF, Ivics Z: Common physical properties of DNA affecting target site selection of sleeping beauty and other Tc1/mariner transposable elements. J Mol Biol. 2002, 323: 441-452. 10.1016/S0022-2836(02)00991-9.
Liu G, Geurts AM, Yae K, Srinivasan AR, Fahrenkrug SC, Largaespada DA, Takeda J, Horie K, Olson WK, Hackett PB: Target-site preferences of Sleeping Beauty transposons. J Mol Biol. 2005, 346: 161-173. 10.1016/j.jmb.2004.09.086.
Bushman F, Lewinski M, Ciuffi A, Barr S, Leipzig J, Hannenhalli S, Hoffmann C: Genome-wide analysis of retroviral DNA integration. Nat Rev Microbiol. 2005, 3: 848-858. 10.1038/nrmicro1263.
Ciuffi A, Llano M, Poeschla E, Hoffmann C, Leipzig J, Shinn P, Ecker JR, Bushman F: A role for LEDGF/p75 in targeting HIV DNA integration. Nat Med. 2005, 11: 1287-1289. 10.1038/nm1329.
Tower J, Karpen GH, Craig N, Spradling AC: Preferential transposition of Drosophila P elements to nearby chromosomal sites. Genetics. 1993, 133: 347-359.
Fischer SE, Wienholds E, Plasterk RH: Regulated transposition of a fish transposon in the mouse germ line. Proc Natl Acad Sci USA. 2001, 98: 6759-6764. 10.1073/pnas.121569298.
Carlson CM, Dupuy AJ, Fritz S, Roberg-Perez KJ, Fletcher CF, Largaespada DA: Transposon mutagenesis of the mouse germline. Genetics. 2003, 165: 243-256.
Luo G, Ivics Z, Izsvak Z, Bradley A: Chromosomal transposition of a Tc1/mariner-like element in mouse embryonic stem cells. Proc Natl Acad Sci USA. 1998, 95: 10769-10773. 10.1073/pnas.95.18.10769.
Dooner HK, Belachew A, Burgess D, Harding S, Ralston M, Ralston E: Distribution of unlinked receptor sites for transposed Ac elements from the bz-m2(Ac) allele in maize. Genetics. 1994, 136: 261-279.
Chen J, Greenblatt IM, Dellaporta SL: Transposition of Ac from the P locus of maize into unreplicated chromosomal sites. Genetics. 1987, 117: 109-116.
Bancroft I, Dean C: Transposition pattern of the maize element Ds in Arabidopsis thaliana. Genetics. 1993, 134: 1221-1229.
Machida C, Onouchi H, Koizumi J, Hamada S, Semiarti E, Torikai S, Machida Y: Characterization of the transposition pattern of the Ac element in Arabidopsis thaliana using endonuclease I-SceI. Proc Natl Acad Sci USA. 1997, 94: 8675-8680. 10.1073/pnas.94.16.8675.
Dooner HK, Keller J, Harper E, Ralston E: Variable patterns of transposition of the maize element activator in tobacco. Plant Cell. 1991, 3: 473-482. 10.1105/tpc.3.5.473.
Belzile F, Yoder JI: Pattern of somatic transposition in a high copy Ac tomato line. Plant J. 1992, 2: 173-179.
Osborne BI, Corr CA, Prince JP, Hehl R, Tanksley SD, McCormick S, Baker B: Ac transposition from a T-DNA can generate linked and unlinked clusters of insertions in the tomato genome. Genetics. 1991, 129: 833-844.
Knapp S, Larondelle Y, Rossberg M, Furtek D, Theres K: Transgenic tomato lines containing Ds elements at defined genomic positions as tools for targeted transposon tagging. Mol Gen Genet. 1994, 243: 666-673.
Kunze R, Weil CF: The hAT and CACTA superfamilies of plant transposons. Mobile DNA II. Edited by: Craig NL, Craigie R, Gellert M, Lambowitz AM. 2002, Washington, DC: ASM Press, 565-610.
Emmons SW, Yesner L, Ruan KS, Katzenberg D: Evidence for a transposon in Caenorhabditis elegans. Cell. 1983, 32: 55-65. 10.1016/0092-8674(83)90496-8.
Liao LW, Rosenzweig B, Hirsh D: Analysis of a transposable element in Caenorhabditis elegans. Proc Natl Acad Sci USA. 1983, 80: 3585-3589. 10.1073/pnas.80.12.3585.
Egilmez NK, Ebert RH, Shmookler Reis RJ: Strain evolution in Caenorhabditis elegans: transposable elements as markers of interstrain evolutionary history. J Mol Evol. 1995, 40: 372-381. 10.1007/BF00164023.
Ketting RF, Plasterk RH: A genetic link between co-suppression and RNA interference in C. elegans. Nature. 2000, 404: 296-298. 10.1038/35005113.
Collins J, Saari B, Anderson P: Activation of a transposable element in the germ line but not the soma of Caenorhabditis elegans. Nature. 1987, 328: 726-728. 10.1038/328726a0.
Bessereau JL, Wright A, Williams DC, Schuske K, Davis MW, Jorgensen EM: Mobilization of a Drosophila transposon in the Caenorhabditis elegans germ line. Nature. 2001, 413: 70-74. 10.1038/35092567.
Bessereau JL: Insertional mutagenesis in C. elegans using the Drosophila transposon Mos1: a method for the rapid identification of mutated genes. Methods Mol Biol. 2006, 351: 59-73.
Mello CC, Kramer JM, Stinchcomb D, Ambros V: Efficient gene transfer in C. elegans: extrachromosomal maintenance and integration of transforming sequences. EMBO J. 1991, 10: 3959-3970.
Berezikov E, Bargmann CI, Plasterk RH: Homologous gene targeting in Caenorhabditis elegans by biolistic transformation. Nucleic Acids Res. 2004, 32: e40-10.1093/nar/gnh033.
Rushforth AM, Saari B, Anderson P: Site-selected insertion of the transposon Tc1 into a Caenorhabditis elegans myosin light chain gene. Mol Cell Biol. 1993, 13: 902-910.
Rushforth AM, Anderson P: Splicing removes the Caenorhabditis elegans transposon Tc1 from most mutant pre-mRNAs. Mol Cell Biol. 1996, 16: 422-429.
Zwaal RR, Broeks A, van Meurs J, Groenen JT, Plasterk RH: Target-selected gene inactivation in Caenorhabditis elegans by using a frozen transposon insertion mutant bank. Proc Natl Acad Sci USA. 1993, 90: 7431-7435. 10.1073/pnas.90.16.7431.
Barrett PL, Fleming JT, Gobel V: Targeted gene alteration in Caenorhabditis elegans by gene conversion. Nat Genet. 2004, 36: 1231-1237. 10.1038/ng1459.
Robert V, Bessereau JL: Targeted engineering of the Caenorhabditis elegans genome following Mos1-triggered chromosomal breaks. EMBO J. 2007, 26: 170-183. 10.1038/sj.emboj.7601463.
Williams DC, Boulin T, Ruaud AF, Jorgensen EM, Bessereau JL: Characterization of Mos1-mediated mutagenesis in Caenorhabditis elegans: a method for the rapid identification of mutated genes. Genetics. 2005, 169: 1779-1785. 10.1534/genetics.104.038265.
Rubin GM, Kidwell MG, Bingham PM: The molecular basis of P-M hybrid dysgenesis: the nature of induced mutations. Cell. 1982, 29: 987-994. 10.1016/0092-8674(82)90462-7.
Bingham PM, Kidwell MG, Rubin GM: The molecular basis of P-M hybrid dysgenesis: the role of the P element, a P-strain-specific transposon family. Cell. 1982, 29: 995-1004. 10.1016/0092-8674(82)90463-9.
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.
Spradling AC: P element-mediated transformation in Drosophila. Drosophila: A Practical Approach. 1986, Oxford-Washington, DC: IRL Press, 175-198.
Kapetanaki MG, Loukeris TG, Livadaras I, Savakis C: High frequencies of Minos transposon mobilization are obtained in insects by using in vitro synthesized mRNA as a source of transposase. Nucleic Acids Res. 2002, 30: 3333-3340. 10.1093/nar/gkf455.
Sarkar A, Atapattu A, Belikoff EJ, Heinrich JC, Li X, Horn C, Wimmer EA, Scott MJ: Insulated piggyBac vectors for insect transgenesis. BMC Biotechnol. 2006, 6: 27-10.1186/1472-6750-6-27.
Gloor GB, Nassif NA, Johnson-Schlitz DM, Preston CR, Engels WR: Targeted gene replacement in Drosophila via P element-induced gap repair. Science. 1991, 253: 1110-1117. 10.1126/science.1653452.
Tsubota S, Schedl P: Hybrid dysgenesis-induced revertants of insertions at the 5' end of the rudimentary gene in Drosophila melanogaster: transposon-induced control mutations. Genetics. 1986, 114: 165-182.
Bier E, Vaessin H, Shepherd S, Lee K, McCall K, Barbel S, Ackerman L, Carretto R, Uemura T, Grell E, et al: Searching for pattern and mutation in the Drosophila genome with a P-lacZ vector. Genes Dev. 1989, 3: 1273-1287. 10.1101/gad.3.9.1273.
Brand AH, Perrimon N: Targeted gene expression as a means of altering cell fates and generating dominant phenotypes. Development. 1993, 118: 401-415.
Hayashi S, Ito K, Sado Y, Taniguchi M, Akimoto A, Takeuchi H, Aigaki T, Matsuzaki F, Nakagoshi H, Tanimura T, et al: GETDB, a database compiling expression patterns and molecular locations of a collection of Gal4 enhancer traps. Genesis. 2002, 34: 58-61. 10.1002/gene.10137.
Friedrich G, Soriano P: Promoter traps in embryonic stem cells: a genetic screen to identify and mutate developmental genes in mice. Genes Dev. 1991, 5: 1513-1523. 10.1101/gad.5.9.1513.
Lukacsovich T, Asztalos Z, Awano W, Baba K, Kondo S, Niwa S, Yamamoto D: Dual-tagging gene trap of novel genes in Drosophila melanogaster. Genetics. 2001, 157: 727-742.
Morin X, Daneman R, Zavortink M, Chia W: A protein trap strategy to detect GFP-tagged proteins expressed from their endogenous loci in Drosophila. Proc Natl Acad Sci USA. 2001, 98: 15050-15055. 10.1073/pnas.261408198.
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.
Rorth P, Szabo K, Bailey A, Laverty T, Rehm J, Rubin GM, Weigmann K, Milan M, Benes V, Ansorge W, et al: Systematic gain-of-function genetics in Drosophila. Development. 1998, 125: 1049-1057.
Bellen HJ, Levis RW, Liao G, He Y, Carlson JW, Tsang G, Evans-Holm M, Hiesinger PR, Schulze KL, Rubin GM, et al: The BDGP gene disruption project: single transposon insertions associated with 40% of Drosophila genes. Genetics. 2004, 167: 761-781. 10.1534/genetics.104.026427.
Spradling AC, Stern D, Beaton A, Rhem EJ, Laverty T, Mozden N, Misra S, Rubin GM: The Berkeley Drosophila Genome Project gene disruption project: single P-element insertions mutating 25% of vital Drosophila genes. Genetics. 1999, 153: 135-177.
Thibault ST, Singer MA, Miyazaki WY, Milash B, Dompe NA, Singh CM, Buchholz R, Demsky M, Fawcett R, Francis-Lang HL, et al: A complementary transposon tool kit for Drosophila melanogaster using P and piggyBac. Nat Genet. 2004, 36: 283-287. 10.1038/ng1314.
Hacker 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.
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.
Gray YH: It takes two transposons to tango: transposable-element-mediated chromosomal rearrangements. Trends Genet. 2000, 16: 461-468. 10.1016/S0168-9525(00)02104-1.
Golic KG: Site-specific recombination between homologous chromosomes in Drosophila. Science. 1991, 252: 958-961. 10.1126/science.2035025.
Ivics Z, Hackett PB, Plasterk RH, Izsvak Z: Molecular reconstruction of Sleeping Beauty, a Tc1-like transposon from fish, and its transposition in human cells. Cell. 1997, 91: 501-510. 10.1016/S0092-8674(00)80436-5.
Ding S, Wu X, Li G, Han M, Zhuang Y, Xu T: Efficient transposition of the piggyBac (PB) transposon in mammalian cells and mice. Cell. 2005, 122: 473-483. 10.1016/j.cell.2005.07.013.
Drabek D, Zagoraiou L, deWit T, Langeveld A, Roumpaki C, Mamalaki C, Savakis C, Grosveld F: Transposition of the Drosophila hydei Minos transposon in the mouse germ line. Genomics. 2003, 81: 108-111. 10.1016/S0888-7543(02)00030-7.
Miskey C, Izsvak Z, Plasterk RH, Ivics Z: The Frog Prince: a reconstructed transposon from Rana pipiens with high transpositional activity in vertebrate cells. Nucleic Acids Res. 2003, 31: 6873-6881. 10.1093/nar/gkg910.
Miskey C, Papp B, Mates L, Sinzelle L, Keller H, Izsvak Z, Ivics Z: The Ancient Mariner sails again: transposition of the human Hsmar1 element by a reconstructed transposase and activities of the SETMAR protein on transposon ends. Mol Cell Biol. 2007, 27: 4589-4600. 10.1128/MCB.02027-06.
Kawakami K, Shima A, Kawakami N: Identification of a functional transposase of the Tol2 element, an Ac-like element from the Japanese medaka fish, and its transposition in the zebrafish germ lineage. Proc Natl Acad Sci USA. 2000, 97: 11403-11408. 10.1073/pnas.97.21.11403.
Raz E, van Luenen HG, Schaerringer B, Plasterk RH, Driever W: Transposition of the nematode Caenorhabditis elegans Tc3 element in the zebrafish Danio rerio. Curr Biol. 1998, 8: 82-88. 10.1016/S0960-9822(98)70038-7.
Fadool JM, Hartl DL, Dowling JE: Transposition of the mariner element from Drosophila mauritiana in zebrafish. Proc Natl Acad Sci USA. 1998, 95: 5182-5186. 10.1073/pnas.95.9.5182.
Nasevicius A, Ekker SC: Effective targeted gene 'knockdown' in zebrafish. Nat Genet. 2000, 26: 216-220. 10.1038/79951.
Sinzelle L, Vallin J, Coen L, Chesneau A, Pasquier DD, Pollet N, Demeneix B, Mazabraud A: Generation of trangenic Xenopus laevis using the Sleeping Beauty transposon system. Transgenic Res. 2006, 15: 751-760. 10.1007/s11248-006-9014-6.
Hamlet MR, Yergeau DA, Kuliyev E, Takeda M, Taira M, Kawakami K, Mead PE: Tol2 transposon-mediated transgenesis in Xenopus tropicalis. Genesis. 2006, 44: 438-445. 10.1002/dvg.20234.
Dupuy AJ, Clark K, Carlson CM, Fritz S, Davidson AE, Markley KM, Finley K, Fletcher CF, Ekker SC, Hackett PB, et al: Mammalian germ-line transgenesis by transposition. Proc Natl Acad Sci USA. 2002, 99: 4495-4499. 10.1073/pnas.062630599.
Wilber A, Frandsen JL, Geurts JL, Largaespada DA, Hackett PB, McIvor RS: RNA as a source of transposase for sleeping beauty-mediated gene insertion and expression in somatic cells and tissues. Mol Ther. 2006, 13: 625-630. 10.1016/j.ymthe.2005.10.014.
Carlson CM, Frandsen JL, Kirchhof N, McIvor RS, Largaespada DA: Somatic integration of an oncogene-harboring Sleeping Beauty transposon models liver tumor development in the mouse. Proc Natl Acad Sci USA. 2005, 102: 17059-17064. 10.1073/pnas.0502974102.
Justice MJ, Noveroske JK, Weber JS, Zheng B, Bradley A: Mouse ENU mutagenesis. Hum Mol Genet. 1999, 8: 1955-1963. 10.1093/hmg/8.10.1955.
Hicks GG, Shi EG, Li XM, Li CH, Pawlak M, Ruley HE: Functional genomics in mice by tagged sequence mutagenesis. Nat Genet. 1997, 16: 338-344. 10.1038/ng0897-338.
Amsterdam A, Burgess S, Golling G, Chen W, Sun Z, Townsend K, Farrington S, Haldi M, Hopkins N: A large-scale insertional mutagenesis screen in zebrafish. Genes Dev. 1999, 13: 2713-2724. 10.1101/gad.13.20.2713.
Kawakami K, Takeda H, Kawakami N, Kobayashi M, Matsuda N, Mishina M: A transposon-mediated gene trap approach identifies developmentally regulated genes in zebrafish. Dev Cell. 2004, 7: 133-144. 10.1016/j.devcel.2004.06.005.
Parinov S, Kondrichin I, Korzh V, Emelyanov A: Tol2 transposon-mediated enhancer trap to identify developmentally regulated zebrafish genes in vivo. Dev Dyn. 2004, 231: 449-459. 10.1002/dvdy.20157.
Davidson AE, Balciunas D, Mohn D, Shaffer J, Hermanson S, Sivasubbu S, Cliff MP, Hackett PB, Ekker SC: Efficient gene delivery and gene expression in zebrafish using the Sleeping Beauty transposon. Dev Biol. 2003, 263: 191-202. 10.1016/j.ydbio.2003.07.013.
Sivasubbu S, Balciunas D, Davidson AE, Pickart MA, Hermanson SB, Wangensteen KJ, Wolbrink DC, Ekker SC: Gene-breaking transposon mutagenesis reveals an essential role for histone H2afza in zebrafish larval development. Mech Dev. 2006, 123: 513-529. 10.1016/j.mod.2006.06.002.
Balciunas D, Davidson AE, Sivasubbu S, Hermanson SB, Welle Z, Ekker SC: Enhancer trapping in zebrafish using the Sleeping Beauty transposon. BMC Genomics. 2004, 5: 62-10.1186/1471-2164-5-62.
Dupuy AJ, Fritz S, Largaespada DA: Transposition and gene disruption in the male germline of the mouse. Genesis. 2001, 30: 82-88. 10.1002/gene.1037.
Horie K, Kuroiwa A, Ikawa M, Okabe M, Kondoh G, Matsuda Y, Takeda J: Efficient chromosomal transposition of a Tc1/mariner-like transposon Sleeping Beauty in mice. Proc Natl Acad Sci USA. 2001, 98: 9191-9196. 10.1073/pnas.161071798.
Zagoraiou L, Drabek D, Alexaki S, Guy JA, Klinakis AG, Langeveld A, Skavdis G, Mamalaki C, Grosveld F, Savakis C: In vivo transposition of Minos, a Drosophila mobile element, in mammalian tissues. Proc Natl Acad Sci USA. 2001, 98: 11474-11478. 10.1073/pnas.201392398.
Horie K, Yusa K, Yae K, Odajima J, Fischer SE, Keng VW, Hayakawa T, Mizuno S, Kondoh G, Ijiri T, et al: Characterization of Sleeping Beauty transposition and its application to genetic screening in mice. Mol Cell Biol. 2003, 23: 9189-9207. 10.1128/MCB.23.24.9189-9207.2003.
Kitada K, Ishishita S, Tosaka K, Takahashi RI, Ueda M, Keng VW, Horie K, Takeda J: Transposon-tagged mutagenesis in the rat. Nat Methods. 2007, 4: 131-133. 10.1038/nmeth1002.
Lu B, Geurts AM, Poirier C, Petit DC, Harrison W, Overbeek PA, Bishop CE: Generation of rat mutants using a coat color-tagged Sleeping Beauty transposon system. Mamm Genome. 2007, 18: 338-346. 10.1007/s00335-007-9025-5.
Geurts AM, Collier LS, Geurts JL, Oseth LL, Bell ML, Mu D, Lucito R, Godbout SA, Green LE, Lowe SW, et al: Gene mutations and genomic rearrangements in the mouse as a result of transposon mobilization from chromosomal concatemers. PLoS Genet. 2006, 2: e156-10.1371/journal.pgen.0020156.
Keng VW, Yae K, Hayakawa T, Mizuno S, Uno Y, Yusa K, Kokubu C, Kinoshita T, Akagi K, Jenkins NA, et al: Region-specific saturation germline mutagenesis in mice using the Sleeping Beauty transposon system. Nat Methods. 2005, 2: 763-769. 10.1038/nmeth795.
Kawakami K, Noda T: Transposition of the Tol2 element, an Ac-like element from the Japanese medaka fish Oryzias latipes, in mouse embryonic stem cells. Genetics. 2004, 166: 895-899. 10.1534/genetics.166.2.895.
Balciunas D, Wangensteen KJ, Wilber A, Bell J, Geurts A, Sivasubbu S, Wang X, Hackett PB, Largaespada DA, McIvor RS, et al: Harnessing a high cargo-capacity transposon for genetic applications in vertebrates. PLoS Genet. 2006, 2: e169-10.1371/journal.pgen.0020169.
Geurts AM, Wilber A, Carlson CM, Lobitz PD, Clark KJ, Hackett PB, McIvor RS, Largaespada DA: Conditional gene expression in the mouse using a Sleeping Beauty gene-trap transposon. BMC Biotechnol. 2006, 6: 30-10.1186/1472-6750-6-30.
Dupuy AJ, Akagi K, Largaespada DA, Copeland NG, Jenkins NA: Mammalian mutagenesis using a highly mobile somatic Sleeping Beauty transposon system. Nature. 2005, 436: 221-226. 10.1038/nature03691.
Collier LS, Carlson CM, Ravimohan S, Dupuy AJ, Largaespada DA: Cancer gene discovery in solid tumours using transposon-based somatic mutagenesis in the mouse. Nature. 2005, 436: 272-276. 10.1038/nature03681.
Dupuy AJ, Jenkins NA, Copeland NG: Sleeping beauty: a novel cancer gene discovery tool. Hum Mol Genet. 2006, 15 (Spec No 1): R75-R79. 10.1093/hmg/ddl061.
Sakharkar M, Passetti F, de Souza JE, Long M, de Souza SJ: ExInt: an exon intron database. Nucleic Acids Res. 2002, 30: 191-194. 10.1093/nar/30.1.191.
Handler AM: Understanding and improving transgene stability and expression in insects for SIT and conditional lethal release programs. Insect Biochem Mol Biol. 2004, 34: 121-130. 10.1016/j.ibmb.2003.08.005.
Osborne BI, Wirtz U, Baker B: A system for insertional mutagenesis and chromosomal rearrangement using the Ds transposon and Cre-lox. Plant J. 1995, 7: 687-701. 10.1046/j.1365-313X.1995.7040687.x.
Hentges KE, Justice MJ: Checks and balancers: balancer chromosomes to facilitate genome annotation. Trends Genet. 2004, 20: 252-259. 10.1016/j.tig.2004.04.004.
Zheng B, Sage M, Cai WW, Thompson DM, Tavsanli BC, Cheah YC, Bradley A: Engineering a mouse balancer chromosome. Nat Genet. 1999, 22: 375-378. 10.1038/11949.
Nishijima I, Mills A, Qi Y, Mills M, Bradley A: Two new balancer chromosomes on mouse chromosome 4 to facilitate functional annotation of human chromosome 1p. Genesis. 2003, 36: 142-148. 10.1002/gene.10207.
Yu Y, Bradley A: Engineering chromosomal rearrangements in mice. Nat Rev Genet. 2001, 2: 780-790. 10.1038/35093564.
Su H, Wang X, Bradley A: Nested chromosomal deletions induced with retroviral vectors in mice. Nat Genet. 2000, 24: 92-95. 10.1038/71756.
Bilodeau M, Girard S, Hebert J, Sauvageau G: A retroviral strategy that efficiently creates chromosomal deletions in mammalian cells. Nat Meth. 2007, 4: 263-268. 10.1038/nmeth1011.
Franz G, Savakis C: Minos, a new transposable element from Drosophila hydei, is a member of the Tc1-like family of transposons. Nucleic Acids Res. 1991, 19: 6646-10.1093/nar/19.23.6646.
Franz G, Loukeris TG, Dialektaki G, Thompson CR, Savakis C: Mobile Minos elements from Drosophila hydei encode a two-exon transposase with similarity to the paired DNA-binding domain. Proc Natl Acad Sci USA. 1994, 91: 4746-4750. 10.1073/pnas.91.11.4746.
Metaxakis A, Oehler S, Klinakis A, Savakis C: Minos as a genetic and genomic tool in Drosophila melanogaster. Genetics. 2005, 171: 571-581. 10.1534/genetics.105.041848.
Jacobson JW, Medhora MM, Hartl DL: Molecular structure of a somatically unstable transposable element in Drosophila. Proc Natl Acad Sci USA. 1986, 83: 8684-8688. 10.1073/pnas.83.22.8684.
Lozovsky ER, Nurminsky D, Wimmer EA, Hartl DL: Unexpected stability of mariner transgenes in Drosophila. Genetics. 2002, 160: 527-535.
O'Hare K, Rubin GM: Structures of P transposable elements and their sites of insertion and excision in the Drosophila melanogaster genome. Cell. 1983, 34: 25-35. 10.1016/0092-8674(83)90133-2.
Fraser MJ, Smith GE, Summers MD: Acquisition of host cell DNA sequences by baculoviruses: relationship between host DNA insertions and FP mutants of Autographa californica and Galleria mellonella nuclear polyhedrosis viruses. J Virol. 1983, 47: 287-300.
Cary LC, Goebel M, Corsaro BG, Wang HG, Rosen E, Fraser MJ: Transposon mutagenesis of baculoviruses: analysis of Trichoplusia ni transposon IFP2 insertions within the FP-locus of nuclear polyhedrosis viruses. Virology. 1989, 172: 156-169. 10.1016/0042-6822(89)90117-7.
Izsvak Z, Ivics Z, Plasterk RH: Sleeping Beauty, a wide host-range transposon vector for genetic transformation in vertebrates. J Mol Biol. 2000, 302: 93-102. 10.1006/jmbi.2000.4047.
Yant SR, Wu X, Huang Y, Garrison B, Burgess SM, Kay MA: High-resolution genome-wide mapping of transposon integration in mammals. Mol Cell Biol. 2005, 25: 2085-2094. 10.1128/MCB.25.6.2085-2094.2005.
Fischer SE, van Luenen HG, Plasterk RH: Cis requirements for transposition of Tc1-like transposons in C. elegans. Mol Gen Genet. 1999, 262: 268-274.
van Luenen HG, Plasterk RH: Target site choice of the related transposable elements Tc1 and Tc3 of Caenorhabditis elegans. Nucleic Acids Res. 1994, 22: 262-269. 10.1093/nar/22.3.262.
Martin E, Laloux H, Couette G, Alvarez T, Bessou C, Hauser O, Sookhareea S, Labouesse M, Segalat L: Identification of 1088 new transposon insertions of Caenorhabditis elegans: a pilot study toward large-scale screens. Genetics. 2002, 162: 521-524.
Collins J, Forbes E, Anderson P: The Tc3 family of transposable genetic elements in Caenorhabditis elegans. Genetics. 1989, 121: 47-55.
Koga A, Suzuki M, Inagaki H, Bessho Y, Hori H: Transposable element in fish. Nature. 1996, 383: 30-10.1038/383030a0.
Urasaki A, Morvan G, Kawakami K: Functional dissection of the Tol2 transposable element identified the minimal cis-sequence and a highly repetitive sequence in the subterminal region essential for transposition. Genetics. 2006, 174: 639-649. 10.1534/genetics.106.060244.
Kotani T, Nagayoshi S, Urasaki A, Kawakami K: Transposon-mediated gene trapping in zebrafish. Methods. 2006, 39: 199-206. 10.1016/j.ymeth.2005.12.006.
This article has been published as part of Genome Biology Volume 8, Supplement 1, 2007: Transposons in vertebrate functional genomics. The full contents of the supplement are available online at http://genomebiology.com/supplements/8/S1
The authors declare that they have no competing interests.
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Mátés, L., Izsvák, Z. & Ivics, Z. Technology transfer from worms and flies to vertebrates: transposition-based genome manipulations and their future perspectives. Genome Biol 8, S1 (2007). https://doi.org/10.1186/gb-2007-8-s1-s1
- Insertional Mutagenesis
- loxP Site
- Sleep Beauty
- Balancer Chromosome
- Gene Trap Vector