We present liquid-cell transmission electron microscopy (liquid-cell TEM) imaging of fixed and non-fixed prostate cancer cells (PC3 and LNCaP) with high resolution in a custom developed silicon nitride liquid cell. Fixed PC3 cells were imaged for 90–120 min without any discernable damage. High contrast on the cellular structures was obtained even at low electron doses (~2.5 e−/nm2 per image). The images show distinct structures of cell compartments (nuclei and nucleoli) and cell boundaries without any further sample embedding, dehydration, or staining. Furthermore, we observed dynamics of vesicles trafficking from the cell membrane in consecutive still frames in a non-fixed cell. Our findings show that liquid-cell TEM, operated at low electron dose, is an excellent tool to investigate dynamic events in non-fixed cells with enough spatial resolution (few nm) and natural amplitude contrast to follow key intracellular processes.

Gene constructs containing the Cauliflower mosaic virus (CaMV) 35S promoter and a sequence coding either for a green fluorescent protein (GFP) or for firefly luciferase were transfected into Chinese hamster ovary (CHO) cells. Both reporter genes were expressed to significant levels. The 35S promoter was 40 times less active than the human eF1α promoter, which is known to be one of the most potent promoters in mammalian cells. The 35S promoter must therefore be considered to be a promoter of significant potency in mammalian cells. RT-PCR analysis suggested that transcription initiation in CHO cells occurred between the TATA box and the transcription start site of the 35S promoter that function in plant cells. Further analysis by 5’RACE confirmed that transcription was initiated in CHO cells at different sites located essentially between the TATA box and the plant transcription start site, showing that 35S promoter activity in animal cells is due to the presence of promoter elements that are functional in mammalian cells, but that are not those used in plants. The data reported here raise the possibility that genes controlled by the 35S promoter, which is commonly used in transgenic plants, have the potential for expression in animal cells.

Small catalytic RNAs like the hairpin ribozyme are proving to be useful intracellular tools; however, most attempts to demonstrate trans-cleavage of RNA by ribozymes in cells have been frustrated by rapid cellular degradation of the cleavage products. Here, we describe a fluorescence resonance energy transfer (FRET) assay that directly monitors cleavage of target RNA in tissue-culture cells. An oligoribonucleotide substrate was modified to inhibit cellular ribonuclease degradation without interfering with ribozyme cleavage, and donor (fluorescein) and acceptor (tetramethylrhodamine) fluorophores were introduced at positions flanking the cleavage site. In simple buffers, the intact substrate produces a strong FRET signal that is lost upon cleavage, resulting in a red-to-green shift in dominant fluorescence emission. Hairpin ribozyme and fluorescent substrate were microinjected into murine fibroblasts under conditions in which substrate cleavage can occur only inside the cell. A strong FRET signal was observed by fluorescence microscopy when substrate was injected, but rapid decay of the FRET signal occurred when an active, cognate ribozyme was introduced with the substrate. No acceleration in cleavage rates was observed in control experiments utilizing a noncleavable substrate, inactive ribozyme, or an active ribozyme with altered substrate specificity. Subsequently, the fluorescent substrates were injected into clonal cell lines that expressed cognate or noncognate ribozymes. A decrease in FRET signal was observed only when substrate was microinjected into cells expressing its cognate ribozyme. These results demonstrate trans-cleavage of RNA within mammalian cells, and provide an experimental basis for quantitative analysis of ribozyme activity and specificity within the cell.

Classical glutathione peroxidase (GPX1) mRNA levels can decrease to less than 10% in selenium (Se)-deficient rat liver. The cis-acting nucleic acid sequence requirements for Se regulation of GPX1 mRNA levels were studied by transfecting Chinese hamster ovary (CHO) cells with GPX1 DNA constructs in which specific regions of the GPX1 gene were mutated, deleted, or replaced by comparable regions from unregulated genes such as phospholipid hydroperoxide glutathione peroxidase (GPX4). For each construct, stable transfectants were pooled two weeks after transfection, divided into Se-deficient (2 nM Se) or Se-adequate (200 nM Se) medium, and grown for an additional four days. On day of harvest, Se-deficient GPX1 and GPX4 activities averaged 13 ± 2% and 15 ± 2% of Se adequate levels, confirming that cellular Se status was dramatically altered by Se supplementation. RNA was isolated from replicate plates of cells and transfected mRNA levels were specifically determined by RNase protection assay. Analysis of chimeric GPX1/GPX4 constructs showed that the GPX4 3′-UTR can completely replace the GPX13′-UTR in Se regulation of GPX1 mRNA. We did not find any GPX1 coding regions that could be replaced by the corresponding GPX4 coding regions without diminishing or eliminating Se regulation of the transfected GPX1 mRNA. Further analysis of the GPX1 coding region demonstrated that the GPX1 Sec codon (UGA) and the GPX1 intron sequences are required for full Se regulation of transfected GPX1 mRNA levels. Mutations that moved the GPX1 Sec codon to three different positions within the GPX1 coding region suggest that the mechanism for Se regulation of GPX1 mRNA requires a Sec codon within exon 1. Lastly, we found that addition of the GPX1 3′-UTR to β-globin mRNA can convey significant Se regulation to β-globin mRNA levels when a UGA codon is placed within exon 1. We conclude that Se regulation of GPX1 mRNA requires a functional selenocysteine insertion sequence (SECIS) in the 3′-UTR and a Sec codon followed by an intron.