Fluorimetric and spectrophotometric studies of DPN-linked isocitrate dehydrogenase from bovine heart. Properties of tyrosyl and tryptophyl residues.

The emission maximum of DPN-linked isocitrate dehydrogenase in pH 7.07 buffer is shifted from 317 to 324 nm and fluorescence intensity is decreased when the excitation wave-length is varied from 270 to 290 nm; in 0.2 M KOH, where the fluorescence of tyrosyl residues is almost completely quenched, a further substantial decline in quantum yield of protein fluorescence and a red shift of the emission peak to 339 nm occur. The latter should be due mainly to tryptophyl residues. The enzyme contains 9.4 tyrosyl residues per subunit of molecular weight 42,000 determined spectrophotometrically (295 nm) at pH 13, in good agreement with a tyrosine content of 9.7 by amino acid analysis. No more than 1.1 tyrosyl residues per subunit can be detected up to pH 10.6 at 7 degrees upon prolonged incubation. The increase in absorption at 295 nm with increasing pH is related to loss of enzyme activity and results in a red shift of the emission maximum, and decreased fluorescence intensity. Treatment of the enzyme in a Li+-containing buffer at pH 7.5 with an excess of N-acetylimidazole results in (a) modification of 1.1 tyrosyl residues per subunit, (b) a 30% decrease in enzyme activity, (c) a 6-nm red shift in emission maximum, and (d) a decrease in fluorescence intensity. Manganous DL-isocitrate (1.06 mM) prevents the acetylation of the enzyme. Deacetylation of the O-acetylated enzyme by hydroxylamine completely restores the enzyme activity and reverses the spectral changes. The acetylation studies indicate that the reactive tyrosyl residue does not participate directly in catalysis but may be involved in maintaining the proper conformation of the active enzyme center. A net of 1 of the 2 tryptophyl residues per subunit is perturbed immediately by a number of solvents. This perturbation is not affected by manganous isocitrate, whereas exposure of tyrosyl residues occurs only with time and is prevented by the substrate. The perturbation of the tryptophyl residue is accompanied by a red shift of the fluorescence emission maximum. The more exposed tryptophyl residue may contribute to the energy transfer from protein to nucleotides since the quenching of protein fluorescence upon binding of DPN+, DPNH, or ADP by enzyme results in a blue shift of the emission maximum. Manganous DL-isocitrate (1.06 mM) quenches protein fluorescence by 16% without a shift in emission peak and does not affect the relative extent of fluorescence quenching induced by the nucleotides.     

Nanosecond pulse fluorometry of conformational change in phenylalanine hydroxylase associated with activation

Conformational change in rat liver phenylalanine hydroxylase associated with activation by phenylalanine or N-(1-anilinonaphth-4-yl)maleimide was investigated by measuring fluorescence spectra and fluorescence lifetimes of tryptophanyl residues as well as the probe fluorophore conjugated with SH groups of the hydroxylase. The fluorescence spectrum of tryptophan exhibited its maximum at 342 nm. It shifted by 8 nm toward longer wavelength accompanied by an increase in its intensity, by preincubation with 1 mM phenylalanine. The fluorescence intensity of tryptophan increased by 36% upon the activation. On the other hand, the binding of (6R)-L-erythro-tetrahydrobiopterin, a natural cofactor of the enzyme, induced a decrease in the fluorescence intensity by 79% without a shift of the maximum wavelength. The fluorescence lifetime of tryptophan of phenylalanine hydroxylase exhibited two components with lifetimes of 1.7 and 4.1 ns. The values of the lifetimes changed to 1.4 and 5.6 ns, respectively, upon the activation. It is considered that the change in the longer lifetime is correlated with the shift of the emission peak upon the activation. The values of both the lifetimes decreased to 0.64 and 3.6 ns upon the binding of (6R)-L-erythro-tetrahydrobiopterin, which is coincident with the decrease in the fluorescence intensity. Conjugation of N-(1-anilinonaphth-4-yl)maleimide with SH of phenylalanine hydroxylase brought about a decrease in both the fluorescence intensity and the value of the shorter lifetime of the tryptophanyl residues, while the longer lifetime remained unchanged.(ABSTRACT TRUNCATED AT 250 WORDS)     

A comparison of the intrinsic fluorescence of red kangaroo, horse and sperm whale metmyoglobins

Several metmyoglobins (red kangaroo, horse and sperm whale), containing different numbers of tyrosines, but with invariant tryptophan residues (Trp-7, Trp-14), exhibit intrinsic fluorescence when studied by steady-state front-face fluorometry. The increasing tyrosine content of these myoglobins correlates with a shift in emission maximum to shorter wavelengths with excitation at 280 nm: red kangaroo (Tyr-146) emission maximum 335 nm; horse (Tyr-103, -146) emission maximum 333 nm; sperm whale (Tyr-103, -146, -151) emission maximum 331 nm. Since 280 nm excites both tyrosine and tryptophan, this strongly suggests that tyrosine emission is not completely quenched but also contributes to this fluorescence emission. Upon titration to pH 12.5, there is a reversible shift of the emission maximum to longer wavelengths with an increase greater than 2-fold in fluorescence intensity. With excitation at 305 nm, a tyrosinate-like emission is detected at a pH greater than 12. These studies show that: (1) metmyoglobins, Class B proteins containing both tyrosine and tryptophan residues, exhibit intrinsic fluorescence; (2) tyrosine residues also contribute to the observed steady-state fluorescence emission when excited by light at 280 nm; (3) the ionization of Tyr-146 is likely coupled to protein unfolding.     

Conformational changes in pennisetin using intrinsic fluorescence spectroscopy

Fluorescence spectra of native pennisetin resulted in a single emission peak at 335 nm at excitation wavelength of 274 and 295 nm with quantum yield values for tyrosine and tryptophan as 0.086 and 0.097, respectively. These results indicate the presence of tryptophan residues in a polar environment and quenching of tyrosine residues in the native state of pennisetin. In the presence of an increasing concentration of guanidine hydrochloride (Gdn · HCl), changes such as red shift in emission peak from 335 to 344 nm, decrease in relative fluorescence intensity and increase in quantum yield value were observed, suggesting unfolding of the pennisetin molecule during denaturation. The quenching of tryptophanyl fluorescence by acrylamide and iodide further showed the presence of a single kind of tryptophanyl residue and its polar environment in pennisetin molecule.     

Interaction of a hydrophobic fluorescent probe with mouse embryo fibroblasts

Fluorescence photomicrographs show that the hydrophobic fluorescent probe 1-anilinonaphthalene-8-sulfonate (ANS) binds to hydrophobic components of intact 3T3 cells. Cells exposed to ANS exhibit fluorescence in the cytoplasm, intense nuclear membrane fluorescence, and well-defined fluorescent nucleoli. Fluorescence titrations of 3T3 cells with ANS show a decrease in fluorescence intensity, a blue shift of native cell emission with increasing ANS concentration and the appearance of a new peak due to ANS fluorescence. These fluorescence effects are ascribed to energy transfer processes involving bound ANS and the tryptophan and tyrosine residues of cellular proteins. ANS bound to 3T3 cells appears to quench the long wavelength component of the cellular tryptophan fluorescence, resulting in an unmasking of tryptophan and tyrosine emission at shorter wavelengths.     

Tryptophan fluorescence studies of plasma fibronectin: effects of environmental factors

Steady state fluorescence measurements have been used to study tryptophan fluorescence of plasma fibronectin. The native protein has an emission maximum at 337 nm with a quantum yield of 0.03. A red shift of emission maximum was observed in 3–5M urea and a further red shift in 7–8M urea. The emission maximum shifted from 337 to 345 nm when the temperature was changed from 30 to 80°C, with a midpoint of thermal denaturation at 58°C. Similarly, the emission maximum shifted from 337 to 345 nm when the solution pH was increased from 9 to 12, with a midpoint of pH transition at 10.6. The results obtained from difference absorption spectroscopy studies suggest that the unfolding of fibronectin at alkaline pH is related at least in part to ionization of tyrosine residues. Since most of the tryptophan residues are in invariant positions in homology sequences, it is suggested here that tryptophan residues are useful intrinsic probes for elucidating fibronectin structure in solution.     

Studies on the temperature effect on bacteriorhodopsin of purple and blue membrane by fluorescence and absorption spectroscopy

Fluorescence and absorption spectra were used to study the temperature effect on theconformation of bacteriorhodopsin (bR) in the blue and purple membranes (termed as bRb and bRprespectively).The maximum emission wavelengths of tryptophan fluorescence in both proteins at roomtemperature are 340 nm,and the fluorescence quantum yield of bRb is about 1.4 fold higher than that of bRp.As temperature increases,the tryptophan fluorescence of bRb decreases,while the tryptophan fluorescenceof bRp increases.The binding study of extrinsic fluorescent probe bis-ANS indicated that the probe can bindonly to bRb,but not to bRp.These results suggest that significant structural difference existed between bRband bRp.It was also found that both kinds of bR are highly thermal stable.The maximum wavelength of theprotein fluorescence emission only shifted from 340 nm to 346 nm at 100℃.More interestingly,as tempera-ture increased,the characteristic absorption peak of bRb at 605 nm decreased and a new absorption peak at380 nm formed.The transition occurred at a narrow temperature range (65℃-70℃).These facts indicatedthat an intermediate can be induced by high temperature.This phenomenon has not been reported before.     

Conformational changes induced by binding of divalent cations to calregulin

Scatchard analysis of equilibrium dialysis studies have revealed that in the presence of 3.0 mM MgCl2 and 150 mM KCl, calregulin has a single binding site for Ca2+ with an apparent dissociation constant (apparent Kd) of 0.05 microM and 14 binding sites for Zn2+ with apparent Kd(Zn2+) of 310 microM. Ca2+ binding to calregulin induces a 5% increase in the intensity of intrinsic fluorescence and a 2-3-nm blue shift in emission maximum. Zn2+ binding to calregulin causes a dose-dependent increase of about 250% in its intrinsic fluorescence intensity and a red shift in the emission maximum of about 11 nm. Half-maximal wavelength shift occurs at 0.4 mol of Zn2+/mol of calregulin, and 100% of the wavelength shift is complete at 2 mol of Zn2+/mol of calregulin. In the presence of Zn2+ and calregulin the fluorescence intensity of the hydrophobic fluorescent probe 8-anilino-1-napthalenesulfonate (ANS) was enhanced 300-400% with a shift in emission maximum from 500 to 480 nm. Half-maximal Zn2+-induced shift in ANS emission maximum occurred at 1.2 mol of Zn2+/mol of calregulin, and 100% of this shift occurred at 6 mol of Zn2+/mol of calregulin. Of 12 cations tested, only Zn2+ and Ca2+ produced changes in calregulin intrinsic fluorescence, and none of these metal ions could inhibit the Zn2+-induced red shift in intrinsic fluorescence emission maximum. Furthermore, none of these cations could inhibit or mimic the Zn2+-induced blue shift in ANS emission maximum. These results suggest that calregulin contains distinct and specific ligand-binding sites for Ca2+ and Zn2+. While Ca2+ binding results in the movement of tryptophan away from the solvent, Zn2+ causes a movement of tryptophan into the solvent and the exposure of a domain with considerable hydrophobic character.     

A rare protein fluorescence behavior where the emission is dominated by tyrosine: case of the 33-kDa protein from spinach photosystem II

An abnormal fluorescence emission of protein was observed in the 33-kDa protein which is one component of the three extrinsic proteins in spinach photosystem II particle (PS II). This protein contains one tryptophan and eight tyrosine residues, belonging to a "B type protein". It was found that the 33-kDa protein fluorescence is very different from most B type proteins containing both tryptophan and tyrosine residues. For most B type proteins studied so far, the fluorescence emission is dominated by the tryptophan emission, with the tyrosine emission hardly being detected when excited at 280 nm. However, for the present 33-kDa protein, both tyrosine and tryptophan fluorescence emissions were observed, the fluorescence emission being dominated by the tyrosine residue emission upon a 280 nm excitation. The maximum emission wavelength of the 33-kDa protein tryptophan fluorescence was at 317 nm, indicating that the single tryptophan residue is buried in a very strong hydrophobic region. Such a strong hydrophobic environment is rarely observed in proteins when using tryptophan fluorescence experiments. All parameters of the protein tryptophan fluorescence such as quantum yield, fluorescence decay, and absorption spectrum including the fourth derivative spectrum were explored both in the native and pressure-denatured forms.     

Quantum dot-antibody and aptamer conjugates shift fluorescence upon binding bacteria

CdSe/ZnS quantum dots (QDs) exhibited fluorescence emission blue shifts when conjugated to antibodies or DNA aptamers that are bound to bacteria. The intensity of the shifted emission peak increased with the number of bound bacteria. Curiously, the emission was consistently shifted to approximately 440-460 nm, which is distinctly different from the major component of the natural fluorescence spectrum of these QDs. This minor emission peak can grow upon conjugation to antibodies or aptamers and subsequent binding to bacterial cell surfaces. We hypothesize that the wavelength shift is due to changes in the chemical environment of the QD conjugates when they encounter the bacterial surface and may be due to physical deformation of the QD that changes the quantum confinement state. Regardless of the mechanism, these remarkable emission wavelength shifts of greater than 140 nm in some cases strongly suggest new applications for QD-receptor conjugates.     

Characterization of reductant-induced, tryptophan fluorescence changes in cytochrome oxidase

We have measured the steady-state tryptophan fluorescence spectrum of cytochrome oxidase in its oxidized and fully reduced states. Reduction of the oxidized enzyme by sodium dithionite causes an apparent shift in the fluorescence emission maximum from 328 nm, in the oxidized enzyme, to 348 nm, in the reduced enzyme. This spectroscopic change has been observed previously and assigned to a redox-linked, conformational change in cytochrome oxidase [Copeland, R. A., Smith, P. A., & Chan, S. I. (1987) Biochemistry 26, 7311-7316]. When dithionite-reduced enzyme sits in an open cuvette, the enzyme returns to the oxidized state, and the fluorescence maximum shifts back to 328 nm. However, the time course of the fluorescence change does not follow the redox state of the enzyme, monitored spectrophotometrically at 445,605, and 820 nm, but follows the disappearance of dithionite, which absorbs at 315 nm. Moreover, when the fluorescence emission spectrum of the dithionite-reduced enzyme is corrected for the absorbance due to dithionite, the fluorescence maximum is found 2 nm blue shifted, relative to that of the oxidized enzyme, at 326 nm. This dithionite-induced, red-shifted steady-state tryptophan fluorescence is also seen with the non-heme-containing enzyme carboxypeptidase A. The tryptophan emission spectrum of untreated carboxypeptidase A is at 332 nm, whereas in the presence of dithionite the emission spectrum of carboxypeptidase A is at 350 nm. When corrected for the absorbance of dithionite, the tryptophan emission maximum is at 332 nm. We have also used the photoreductant 3,10-dimethyl-5-deazaisoalloxazine (deazaflavin) to reduce cytochrome oxidase.(ABSTRACT TRUNCATED AT 250 WORDS)     

Decay-associated fluorescence spectra and the heterogeneous emission of alcohol dehydrogenase

A procedure is described for using nanosecond time resolved fluorescence decay data to obtain decay-associated fluorescence spectra. It is demonstrated that the individual fluorescence spectra of two or more components in a mixture can be extracted without prior knowledge of their spectral shapes or degree of overlap. The procedure is also of value for eliminating scattered light artifacts in the fluorescence spectra of turbid samples. The method was used to separate the overlapping emission spectra of the two tryptophan residues in horse liver alcohol dehydrogenase. Formation of a ternary complex between the enzyme, NAD+, and pyrazole leads to a decrease in the total tryptophan fluorescence. It is shown that the emission of both tryptophan residues decreases. The buried tryptophan (residue 314) undergoes dynamic quenching with no change in the spectral distribution. Under the same conditions, the fluorescence intensity of tryptophan (residue 15) decreases without a change in decay time but with a red shift of the emission spectrum. There is also a decrease in tryptophan fluorescence intensity when the free enzyme is acid denatured (succinate buffer, pH 4.1). The denatured enzyme retains sufficient structure to provide different microenvironments for different tryptophan residues as reflected by biexponential decay and spectrally shifted emission spectra (revealed by decay association). The value of this technique for studies of microheterogeneity in biological macromolecules is discussed.     

Tryptophan fluorescence of terminal deoxynucleotidyl transferase: effects of quenchers on time-resolved emission spectra

Terminal deoxynucleotidyl transferase (EC 2.7.7.31) is a eucaryotic DNA polymerase that does not require a template. The tryptophan environments in calf thymus terminal transferase were investigated by fluorescence. The heterogeneous emission from this multitryptophan enzyme was separated by time-resolved emission spectroscopy. Nanosecond fluorescence decays at 296-nm excitation and various emission wavelengths were deconvolved by global analysis, assuming that the lifetimes but not the relative weighting factors were independent of emission wavelength. The data were fit to three exponentials of lifetimes tau 1 = 1.4 ns, tau 2 = 4.5 ns, and tau 3 = 7.7 ns. The corresponding decay-associated emission spectra of the three components had maxima at about 328, 335, and 345 nm. The accessibility of individual tryptophan environments to polar and nonpolar fluorescence quenchers was examined in steady-state and time-resolved experiments. In the presence of iodide and acrylamide, the steady-state emission spectra shift to the blue. However, at low quencher concentrations, the emission from the 7.7-ns component (maximum 345 nm) is hardly affected, suggesting that this hydrophilic tryptophan environment is buried within the protein. On the other hand, the red shift in the steady-state emission spectrum in the presence of trichloroethanol indicates that the 1.4-ns component (maximum 328 nm) is an exposed hydrophobic tryptophan environment. The results are consistent with an inside-out model for terminal transferase protein, with the more hydrophobic tryptophan(s) near the surface and the most hydrophilic tryptophan(s) in the core.     

Conformational and activity changes during guanidine denaturation of D-glyceraldehyde-3-phosphate dehydrogenase

Changes in intrinsic protein fluorescence of lobster muscle D-glyceraldehyde-3-phosphate dehydrogenase (D-glyceraldehyde-3-phosphate: NAD+ oxidoreductase (phosphorylating), EC 1.2.1.12) have been compared with inactivation of the enzyme during denaturation in guanidine solutions. The holoenzyme is completely inactivated at guanidine concentrations less than 0.5 M and this is accompanied by a red shift of the emission maximum at 335 nm and a marked decrease in intensity of the intrinsic fluorescence. At 0.5 M guanidine, the inactivation is a slow process, with a first-order rate constant of 2.4 X 10(-3) s-1. A further red shift in the emission maximum and a decrease in intensity occur at guanidine concentrations higher than 1.5 M. The emission peak at 410 nm of the fluorescent NAD derivative introduced at the active site of this enzyme (Tsou, C.L. et al. (1983) Biochem. Soc. Trans. 11, 425-429) shows both a red shift and a marked decrease in intensity at the same guanidine concentration required to bring about the inactivation and the initial changes in the intrinsic fluorescence of the holoenzyme. It appears that treatment by low guanidine concentrations leads to both complete inactivation and perturbation of the active site conformation and that a tryptophan residue is situated at or near the active site.     

An unusual fluorescence spectrum of a protein proteinase inhibitor, Streptomyces subtilisin inhibitor.

Streptomyces subtilisin inhibitor, a dimeric protein proteinase inhibitor isolated in crystalline form by Murae et al. in 1972, contains three tyrosine and one tryptophan residues per monomer unit and has unusual fluorescence properties. When excited at 280 nm, it shows a characteristic fluorescence spectrum having a peak at 307 nm and a shoulder near 340 nm, a feature which has been recognized only for a very few cases in proteins containing both tryosine and tryptophan residues. When excited at 295 nm, at which tryrosine scarcely absorbs, the inhibitor shows an emission spectrum with a peak at 340 nm characteristic of a tryptophan residue. The emission with a peak at 307 nm is considered to arise from the tryrosine residues. The tryptophan quantum yield of Streptomyces subtilisin inhibitor excited at 295 nm is very small, indicating that the tryptophan florescence is strongly quenched in the native state of the inhibitor. Below pH 4 the peak of the fluorescence spectrum of the inhibitor excited at 280 nm shifts toward 340-350 nm with a concomitant increase in the quantum yield. The structural change induced by low pH seems to release the tryptophan fluorescence from the quenching.     

Immunoaffinity purification and fluorescence studies of human adenosine deaminase

Human thymus adenosine deaminase was isolated by using a monoclonal antibody affinity column. The highly purified enzyme produced by this rapid, efficient procedure had a molecular weight of 44,000. Quenching of the intrinsic protein fluorescence by small molecules was used to probe the accessibility of tryptophan residues in the enzyme and enzyme-inhibitor complexes. The fluorescence emission spectrum of human adenosine deaminase at 295-nm excitation had a maximum at about 335 nm and a quantum yield of 0.03. Addition of polar fluorescence quenchers, iodide and acrylamide, shifted the peak to the blue, and the hydrophobic quencher trichloroethanol shifted the peak to the red, indicating that the emission spectrum is heterogeneous. The fluorescence quenching parameters obtained for these quenchers reveal that the tryptophan environments in the protein are relatively hydrophobic. Binding of both ground-state and transition-state analogue inhibitors caused decreases in the fluorescence intensity of the enzyme, suggesting that one or more tryptophans may be near the active site. The kinetics of the fluorescence decrease were consistent with a slow conformational alteration in the transition-state inhibitor complexes. Fluorescence quenching experiments using polar and nonpolar quenchers were also carried out for the enzyme-inhibitor complexes. The quenching parameters for all enzyme-inhibitor complexes differed from those for the uncomplexed enzyme, suggesting that inhibitor binding causes changes in the conformation of adenosine deaminase. For comparison, parallel quenching studies were performed for calf adenosine deaminase in the absence and presence of inhibitors. While significant structural differences between adenosine deaminase from the two sources were evident, our data indicate that both enzymes undergo conformational changes on binding ground-state and transition-state inhibitors.     

Interaction of lipoprotein lipase and apolipoprotein C-II with sonicated vesicles of 1,2-ditetradecylphosphatidylcholine: comparison of binding constants

The interaction of lipoprotein lipase (LpL) and its activator protein, apolipoprotein C-II (apoC-II), with a nonhydrolyzable phosphatidylcholine, 1,2-ditetradecyl-rac-glycero-3-phosphocholine (C14-ether-PC), was studied by fluorescence spectroscopy. A complex of 320 molecules of C14-ether-PC per LpL was isolated by density gradient ultracentrifugation in KBr. The intrinsic tryptophan fluorescence emission spectrum of LpL was shifted from 336 nm in the absence of lipid to 330 nm in the LpL-lipid complex; the shift was associated with a 40% increase in fluorescence intensity. Addition of C14-ether-PC vesicles to apoC-II caused a 2.5-fold increase in intrinsic tryptophan fluorescence and a shift in emission maximum from 340 to 317 nm. LpL and apoC-II/C14-ether-PC stoichiometries and binding constants were determined by measuring the increase in the intrinsic tryptophan fluorescence as a function of lipid and protein concentrations; for LpL the rate and magnitude of the fluorescence increases were relatively independent of temperature in the range 4-37 degrees C. A stoichiometry of 270 PC per LpL for the LpL-lipid complex compares favorably with the value obtained in the isolated complex. The dissociation constant (Kd) of the complex is 4.3 X 10(-8) M. For apoC-II, the stoichiometry of the complex is 18 PC per apoprotein, and the Kd is 3.0 X 10(-6) M. These data suggest that LpL binds more strongly than apoC-II to phosphatidylcholine interfaces.     

Myelin basic protein interaction with zinc and phosphate: fluorescence studies on the water-soluble form of the protein.

The interaction of myelin basic protein (MBP) with zinc and phosphate ions has been studied by using the emission properties of the single tryptophan residue of the protein (Trp-115). The studies have been carried out by means of both static and time-resolved fluorescence techniques. The addition of either zinc to MBP in the presence of phosphate or phosphate to MBP in the presence of zinc resulted in an increase of fluorescence intensity and a blue shift of the emission maximum wavelength. Furthermore, a concomitant increase in the scattering was also detected. Anisotropy decay experiments demonstrated that these effects are due to the formation of MBP molecules into large aggregates. A possible physiological role for such interaction is discussed.     

Localization of polyphosphates in Saccharomyces fragilis, as revealed by 4′,6-diamidino-2-phenylindole fluorescence

The fluorescent dye 4′,6-diamidino-2-phenylindole has its emission maximum at 456 nm. Fluorescence intensity at this wavelength is significantly increased by various negatively-charged polyelectrolytes. Among several polyelectrolytes tested, polyphosphates appeared to be unique in the sense that they shifted the emission maximum from 456 to 526 nm. Addition of Saccharomyces fragilis cells to a diamidinophenylindole solution caused an immediate shift of the emission maximum to 526 nm, followed by a gradual increase of fluorescence at 456 nm. The 526 nm, but not the 456 nm fluorescence was instantly quenched by non-penetrating cations, like UO²⁺₂. These results suggest a momentary interaction of diamidinophenylindole with polyphosphate, localized outside the plasma membrane, followed by a slow penetration of the dye into the cells, yielding increased fluorescence at 456 nm by interaction of the dye with e.g., nucleic acids. This was confirmed by fluorescence microscopy. After addition of diamidinophenylindole the yeast cells exhibited an immediate green-yellow fluorescence of the membrane, that was suppressed by UO²⁺₂. After longer incubation times the cytoplasm and nucleus developed a blue fluorescence.     

The interaction of Abrus precatorius agglutinin with saccharides as analyzed by fluorescence spectroscopy

The binding of saccharides to Abrus precatorius agglutinin (APA) was analyzed by fluorescence spectroscopy. Upon binding of specific saccharides, the fluorescence emission maximum of APA (338 nm) shifted to shorter wavelength by 5 nm, owing to the change in the environment of tryptophan. By analyzing the change in the fluorescence intensity at 338 nm as a function of concentration of saccharides, the association constants for binding of saccharides to APA were determined. The results suggest that in the saccharide binding site on each B-chain of APA, there may be a site which interacts with the saccharide residue linked to galactopyranoside at the non-reducing end, in addition to the site which recognizes the galactopyranosyl residue. Fluorescence quenching data indicate that 8 out of 24 tryptophans in APA are located at or near the surface of the protein molecule and are available for quenching with both KI and acrylamide, and 10 tryptophans are involved in the environment to which acrylamide has access but KI does not. Binding of lactose to APA reduced by 4 the number of tryptophan residues accessible to quenchers. Based on the results, it is suggested that the tryptophan residues at the saccharide binding site on each B-chain of APA are present on the surface of the APA molecule, and they are shielded from quenching by KI and acrylamide upon binding with specific saccharides.