Cell-penetrating peptides (CPPs) are cationic peptides which, when linked to genes, proteins, or nanoparticles, facilitate the transport of these entities across the cell membrane. Despite their potential use for gene transfer and drug delivery, the mode of action of CPPs is still mysterious. It has even been argued that the observed transport across the cell membrane is an artifact caused by chemical fixation of the cells, a common preparation method for microscopic observation. Here we have synthesized a fluorescent derivative of the HIV-1 TAT protein transduction domain [Fg-CPP(TAT(PTD))] and have observed its uptake into nonfixated living fibroblasts with time-lapse confocal microscopy, eliminating the need for fixation. We observe that Fg-CPP(TAT(PTD)) enters the cytoplasm and nucleus of nonfixated fibroblasts within seconds, arguing against the suggested artifact of cell fixation. Using differential interference contrast microscopy, dense aggregates are detected on the cell surface. Several observations suggest that these aggregates consist of Fg-CPP(TAT(PTD)) bound to membrane-associated heparan sulfate (HS). The aggregates grow in parallel with Fg-CPP(TAT(PTD)) uptake and are detected only on fibroblasts showing Fg-CPP(TAT(PTD)) uptake. These observations resemble earlier reports of "capping" of cell surface molecules combined with a polarized endocytotic flow. Enzymatic removal of extracellular HS reduced the rate of both Fg-CPP(TAT(PTD)) uptake and aggregate formation, demonstrating that HS is involved in the uptake mechanism. The functionality of the fibroblasts during the CPP uptake was investigated with a cytosensor microphysiometer measuring the extracellular acidification rate (ECAR). Short exposures (2.5 min) to the CPP reduced the ECAR which was, however, reversible upon reperfusion with buffer only. In contrast, no recovery to baseline values was observed after repeated exposures to the CPP, suggesting that the CPP is toxic in long-term applications.

We assessed the interaction of three electrically neutral detergents (Triton X-100, C(12)EO(8), and Tween 80) with P-glycoprotein (ABCB1, MDR1) and identified the molecular elements responsible for this interaction. To this purpose we titrated P-glycoprotein in inside-out plasma membrane vesicles of MDR1-transfected mouse embryo fibroblasts (NIH-MDR1-G185) with the detergents below their critical micelle concentration, CMC. The P-glycoprotein ATPase measured as a function of the detergent concentration yielded bell-shaped activity curves which were evaluated with a two-site binding model. The lipid-water partition coefficient and the transporter-water binding constant of the detergents were measured independently. Knowledge of these two parameters allowed assessment of the free energy of detergent binding to P-glycoprotein in the lipid membrane, DeltaG(tl)(0), that reflects the direct detergent-transporter affinity. It increased as the number of ethoxyl groups increased, suggesting that these hydrogen bond acceptor groups are the key elements for the detergent-transporter interaction in the lipid membrane. The free energy of binding to P-glycoprotein per ethoxyl group (EO) was determined as approximately DeltaG(EO)(0)=-1.6 kJ/mol. The present findings moreover document that, depending on the concentration applied, detergents are intrinsic substrates for, or inhibitors of P-glycoprotein.

Extracellular acidification rates (ECARs) in response to eight different drugs activating or inhibiting the ATPase of P-glycoprotein (Pgp) were measured in real time by means of a Cytosensor microphysiometer in MDR1-transfected and corresponding wild-type cell lines, i.e., pig kidney cells (LLC-MDR1 and LLC-PK1) and mouse embryo fibroblasts (NIH-MDR-G185 and NIH3T3). The ECARs showed a bell-shaped dependence on drug concentration (log scale) in transfected cells but were negligibly small in wild-type cells. The activation profiles (ECARs vs concentration) were analyzed in terms of a model assuming activation of Pgp-ATPase with one and inhibition with two drug molecules bound. The kinetic constants [concentration of half-maximum activation (inhibition), K(i), and the maximum (minimum) transporter activity, V(i)] were in qualitative and quantitative agreement with those determined earlier for Pgp-ATPase activation monitored by phosphate release in inside-out cellular vesicles and in purified reconstituted systems, respectively. Furthermore, the ECARs correlated with the expression level of Pgp in the two different cell lines and were reduced in a concentration-dependent manner by cyclosporin A, a potent inhibitor of the Pgp-ATPase. In contrast, treatment of cells with inhibitors of the Na(+)/H(+) or the Cl(-)/HCO(3)(-) exchanger did not reduce the ECARs. The micro-pH measurements provide for the first time direct evidence for a tight coupling between the rate of extracellular proton extrusion and intracellular phosphate release upon Pgp-ATPase activation. They support a Pgp-mediated transport of protons from the site of ATP hydrolysis to the cell surface. Measurement of the ECARs could thus constitute a new method to conveniently analyze the kinetics of Pgp-ATPase activation in living cells.

We compared the P-glycoprotein ATPase activity in inside-out plasma membrane vesicles and living NIH-MDR1-G185 cells with the aim to detect substrate transport. To this purpose we used six substrates which differ significantly in their passive influx through the plasma membrane. In cells, the cytosolic membrane leaflet harboring the substrate binding site of P-glycoprotein has to be approached by passive diffusion through the lipid membrane, whereas in inside-out plasma membrane vesicles, it is accessible directly from the aqueous phase. Compounds exhibiting fast passive influx compared to active efflux by P-glycoprotein induced similar ATPase activity profiles in cells and inside-out plasma membrane vesicles, because their concentrations in the cytosolic leaflets were similar. Compounds exhibiting similar influx as efflux induced in contrast different ATPase activity profiles in cells and inside-out vesicles. Their concentration was significantly lower in the cytosolic leaflet of cells than in the cytosolic leaflet of inside-out membrane vesicles, indicating that P-glycoprotein could cope with passive influx. P-glycoprotein thus transported all compounds at a rate proportional to ATP hydrolysis (i.e. all compounds were substrates). However, it prevented substrate entry into the cytosol only if passive influx of substrates across the lipid bilayer was in a similar range as active efflux.

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