Two retrovirus promoter trap vectors (U3His and U3Neo) have been used to disrupt genes expressed in totipotent murine embryonal stem (ES) cells. Selection in L-histidinol or G418 produced clones in which the coding sequences for histidinol-dehydrogenase or neomycin-phosphotransferase were fused to sequences in or near the 5' exons of expressed genes, including one in the developmentally regulated REX-1 gene. Five of seven histidinol-resistant clones and three of three G418-resistant clones generated germ-line chimeras. A total of four disrupted genes have been passed to the germ line, of which two resulted in embryonic lethalities when bred to homozygosity. The ability to screen large numbers of recombinant ES cell clones for significant mutations, both in vitro and in vivo, circumvents genetic limitations imposed by the size and long generation time of mice and will facilitate a functional analysis of the mouse genome.

A strategy employing gene-trap mutagenesis and site-specific recombination (Cre/ loxP ) has been developed to isolate genes that are transcriptionally activated during programmed cell death. Interleukin-3 (IL-3)-dependent hematopoietic precursor cells (FDCP1) expressing a reporter plasmid that codes for herpes simplex virus–thymidine kinase, neomycin phosphotransferase, and murine IL-3 were transduced with a retroviral gene-trap vector carrying coding sequences for Cre-recombinase (Cre) in the U3 region. Activation of Cre expression from integrations into active genes resulted in a permanent switching between the selectable marker genes that converted the FDCP1 cells to factor independence. Selection for autonomous growth yielded recombinants in which Cre sequences in the U3 region were expressed from upstream cellular promoters. Because the expression of the marker genes is independent of the trapped cellular promoter, genes could be identified that were transiently induced by IL-3 withdrawal.

No abstract