Human RNase H1 activity is regulated by a unique redox switch formed between adjacent cysteines.

Human RNase H1 is active only under reduced conditions. Oxidation as well as N-ethylmaleimide (NEM) treatment of human RNase H1 ablates the cleavage activity. The oxidized and NEM alkylated forms of human RNase H1 exhibited binding affinities for the heteroduplex substrate comparable with the reduced form of the enzyme. Mutants of human RNase H1 in which the cysteines were either deleted or substituted with alanine exhibited cleavage rates comparable with the reduced form of the enzyme, suggesting that the cysteine residues were not required for catalysis. The cysteine residues responsible for the observed redox-dependent activity of human RNase H1 were determined by site-directed mutagenesis to involve Cys(147) and Cys(148). The redox states of the Cys(147) and Cys(148) residues were determined by digesting the reduced, oxidized, and NEM-treated forms of human RNase H1 with trypsin and analyzing the cysteine containing tryptic fragments by micro high performance liquid chromatography-electrospray ionization-Fourier transform ion cyclotron mass spectrometry. The tryptic fragment Asp(131)-Arg(153) containing Cys(147) and Cys(148) was identified. The mass spectra for the Asp(131)-Arg(153) peptides from the oxidized and reduced forms of human RNase H1 in the presence and absence of NEM showed peptide masses consistent with the formation of a disulfide bond between Cys(147) and Cys(148). These data show that the formation of a disulfide bond between adjacent Cys(147) and Cys(148) residues results in an inactive enzyme conformation and provides further insights into the interaction between human RNase H1 and the heteroduplex substrate.