Construction of a fluorescent biosensor family



Bacterial periplasmic binding proteins (bPBPs) are specific for a wide variety of small molecule ligands. bPBPs undergo a large, ligand-mediated conformational change that can be linked to reporter functions to monitor ligand concentrations. This mechanism provides the basis of a general system for engineering families of reagentless biosensors that share a common physical signal transduction functionality and detect many different analytes. We demonstrate the facility of designing optical biosensors based on fluorophore conjugates using 8 environmentally sensitive fluorophores and 11 bPBPs specific for diverse ligands, including sugars, amino acids, anions, cations, and dipeptides. Construction of reagentless fluorescent biosensors relies on identification of sites that undergo a local conformational change in concert with the global, ligand-mediated hinge-bending motion. Construction of cysteine mutations at these locations then permits site-specific coupling of environmentally sensitive fluorophores that report ligand binding as changes in fluorescence intensity. For 10 of the bPBPs presented in this study, the three-dimensional receptor structure was used to predict the location of reporter sites. In one case, a bPBP sensor specific for glutamic and aspartic acid was designed starting from genome sequence information and illustrates the potential for discovering novel binding functions in the microbial genosphere using bioinformatics.

Biosensors are analytical tools that measure the presence of a single molecular species in complex mixtures by combining the exquisite molecular recognition properties of biological macromolecules with signal transduction mechanisms that couple ligand binding to readily detectable physical changes (Hall 1991; Scheller et al. 2001). Ideally, a biosensor is reagentless and does not change composition as a consequence of making the measurement (Hellinga and Marvin 1998), unlike enzyme-based assays or competitive immunoassays, for instance. Most biosensors combine a naturally occurring macromolecule such as an enzyme or an antibody, with the identification of a suitable physical signal particular to the molecule in question, and the construction of a detector specific to that system (Meadows 1996). Recently, molecular engineering techniques have been explored to develop macromolecules that combine a wide range of binding specificities and affinities with a common signal transduction mechanism, to construct a generic detection system for many different analytes (Hellinga and Marvin 1998). Here we demonstrate that protein engineering techniques, based on straightforward structural principles, can be used systematically to adapt the bacterial periplasmic binding proteins (bPBPs) into a versatile biosensor system that combines the large, natural ligand-binding diversity found within this superfamily with generic, reagentless, engineered signal transduction mechanisms. We demonstrate that the biodiversity of this superfamily can be readily exploited to generate biosensors for a wide variety of chemical classes with widespread potential utility (Table 1), including sugars, amino acids, dipeptides, cations, and anions.

Escherichia coli bPBPs are members of a protein superfamily (Tam and Saier Jr. 1993) that is proving to be well suited for the engineering of biosensors. These proteins consist of two domains linked by a hinge region (Quiocho and Ledvina 1996). The ligand-binding site is located at the interface between the two domains. The proteins typically adopt two conformations: a ligand-free open form and a liganded closed form, which interconvert via a hinge-bending mechanism upon ligand binding. This global, ligand-mediated conformational change has been exploited to couple ligand binding to changes in fluorescence intensity by positioning single, environmentally sensitive fluorophores in locations that undergo local conformational changes in concert with the global change (Brune et al. 1994; Gilardi et al. 1994, 1997; Marvin et al. 1997; Marvin and Hellinga 1998, 2001a; Tolosa et al. 1999; Dattelbaum and Lakowicz 2001; Salins et al. 2001). Conformational coupling mechanisms can also be devised to alter the flow of current between the surface of an electrode derivatized with the engineered bPBP containing a covalently attached redox cofactor (Benson et al. 2001). These engineered conformational coupling mechanisms allow reagentless optical and electrochemical biosensors to be constructed using the bPBPs.

The engineered conformational coupling mechanisms are universal to all bPBPs that undergo a ligand-mediated hinge-bending motion and should therefore permit modular manipulation of ligand-binding specificity and affinity, as the reporter group and ligand-binding sites can be sterically separated (Marvin et al. 1997; Marvin and Hellinga 1998). Using engineered maltose-binding protein (maltose BP), we have previously demonstrated that specificity can be radically changed without destroying the reagentless optical (Marvin and Hellinga 2001a) or electrochemical (Benson et al. 2001) signal transduction mechanism. Similarly the ligand-binding affinity can be drastically altered in maltose BP with retention of the conformational coupling mechanism (Marvin et al. 1997; Marvin and Hellinga 2001a). Here we present an investigation into the universality of the engineered conformational coupling mechanism. We have used 10 bPBPs of known structure and introduced 8 different environmentally sensitive fluorophores at a variety of locations predicted to link local conformational changes to the global, ligand-mediated hinge-bending motion. Furthermore, we show that bioinformatics techniques can be used to predict the location of linked sites in bPBPs whose structure is not known, thereby opening opportunities for using the large number of paralogs and homologs that have recently been identified in this family by genomic sequencing studies (Blattner et al. 1997; Quentin et al. 1999). Together with the opportunities of structure-based redesign of ligand-binding specificity (Hellinga and Richards 1991; Marvin and Hellinga 2001a; M.A. Dwyer, L.L. Looger, J.J. Smith, and H.W. Hellinga, unpubl.; L.L. Looger, M.A. Dwyer, J.J. Smith, and H.W. Hellinga, unpubl.), these studies demonstrate the vast potential of the bPBP superfamily as the basis for a system of biosensors suited to a broad range of applications.


Family of biosensors

A set of 11 bPBPs with widely varying ligand-binding specificities was selected for engineering biosensor function (Table 2). All were from E. coli except Fe(III) BP, which is from Haemophilus influenzae. Binding specificities and affinities of these proteins for their respective ligands have been characterized (references in Table 2). Three proteins bind monosaccharides (arabinose, glucose, and ribose BP), one binds di- and trisaccharides of glucose (maltose BP), three bind amino acids (glutamate/aspartate, histidine, and glutamine BP), one binds di- and tripeptides (dipeptide BP), two bind oxyanions (phosphate and sulfate BP), and one binds a metal ion [Fe(III) BP]. Most of these bPBPs bind at most two or three related ligands with high affinity (micromolar or better). For example, phosphate BP binds phosphate and arsenate but not other oxyanions (Luecke and Quiocho 1990), and glucose BP binds glucose and galactose but not other monosaccharides (Anraku 1968). Dipeptide BP is an exception in that it binds a wide variety of di- and tripeptides (Smith et al. 1999). Measured ligand dissociation constants in these proteins are typically in the range of 0.1–1 μM. An exception is Fe(III) BP, where the Kd for Fe(III)(aq) is estimated to be 10−21 M in competition assays with Fe(III) chelates (Adhikari et al. 1995).

For 9 of the 11 proteins selected for this study crystal structures have been solved of the closed, ligand-bound state (Table 2). In the case of sulfate BP, the crystal structure of the E. coli protein has not been reported, so that of Salmonella typhimurium sulfate BP was adopted to model the E. coli protein. Sulfate BP from E. coli and S. typhimurium are 95% identical in amino acid sequence and hence likely to have highly similar structures, in analogy to histidine BP from these two organisms (Oh et al. 1994; Yao et al. 1994). Structures have been solved for the open unliganded state for 6 of the 11 proteins as well (Table 2).

Structure-based design of conformational coupling

Linkage between ligand binding and change in fluorescence of a covalently coupled environmentally sensitive fluorophore can be established if the local environment of the fluorophore changes in concert with formation of the complex. Two mechanisms can be distinguished to establish such structural linkage relationships. Direct linkage involves formation of a nonbonded contact between the bound ligand and the conjugated fluorophore. Indirect linkage involves changes in the local protein structure in the immediate vicinity of the attached fluorophore, and relies on ligand-mediated conformational changes such as the hinge-bending motion observed in the bPBPs.

Direct linkage relationships are readily designed by replacing a residue known to form a ligand contact with a cysteine to which the fluorophore is attached (“endosteric” attachment site). Indirect linkage relationships can be established in two ways. The most straightforward method relies on visual inspection of the ligand complex structure and identifying residues that are located in the vicinity of the binding site but do not interact directly with the ligand and that are likely to be involved in conformational changes. In the case of the bPBPs such are residues located at the perimeter of the interdomain cleft that forms the ligand binding site. The environment of these “peristeric” sites changes significantly upon formation of the closed state. The second approach identifies sites in the protein structure that are located some distance away from the ligand-binding site and undergo a local conformational change in concert with ligand binding. If the structures of both the open and closed states are known, then such “allosteric” sites can be identified using a computational method that analyzes the conformational change (Marvin et al. 1997). Alternatively, once allosteric sites have been identified in one bPBP, structural homology arguments can be invoked to identify such sites in other bPBPs in which only one state has been characterized (Marvin and Hellinga 1998). Table 3 summarizes the designs of all three classes of sites in each of the receptors used in this study. The locations of these sites in the 11 bPBPs are shown in Figure 1.

Sequence-based design of conformational coupling

The number of bPBPs of known sequence greatly exceeds the number for which structures have been solved or for which functions have been assigned by genetic or biochemical characterization. To exploit this reservoir of potential biosensors, coding sequences for bPBPs must be identified and their putative ligand-binding specificities must be established. The identification of bPBPs in microbial genomes relies on finding amino acid sequence homologies to particular clusters of the bPBP family (Tam and Saier 1993). Ligand-binding can then be determined by direct experimentation or be inferred either by structural relationships to bPBPs of known function or by establishing genetic linkage to other genes of known function (Pellegrini et al. 1999). Subsequently, sites within the homolog that undergo local conformational change, and to which reporter functions can be attached, must be identified. The selection of sites for attaching reporter functions relies on homology to bPBPs of known structure.

To illustrate these principles we sought to construct a glutamate biosensor starting from genome sequence data only. The genome of E. coli K12 contains the locus ybeJ encoding a protein identified as a putative bPBP based on amino acid sequence homology with glutamine and histidine BPs (26% and 23% sequence identity; 41% and 43% sequence similarity, respectively) (Blattner et al. 1997). The assignment of YBEJ as an amino acid-binding protein was strengthened by the presence of conserved residues found to be associated with binding to the α-amino and α-carboxylate groups of the ligand in all bPBP amino acid-binding proteins of known structure identified in E. coli (Table 4). Of additional interest is the presence of an arginine residue in YBEJ located at a position that in the other amino acid-binding proteins interacts directly with the side chain of the bound amino acid, suggesting that YBEJ binds an amino acid bearing a negatively charged side chain. Finally, ybeJ is located adjacent to three tandem genes (gltJ, gltK, gltL) postulated to be involved in the glutamate/aspartate transport system (Lum and Wallace 1995 GenBank Accession No. U10981), suggesting that ybeJ encodes a glutamate/aspartate BP. Putative allo-, endo-, and peristeric sites were identified from a structure-based sequence alignment of YBEJ with glutamine BP and histidine BP (Fig. 2).

Mutagenesis and protein production

All of the genes for the bPBPs used in this study were cloned from E. coli or H. influenzae genomic DNA using PCR. The leader peptide sequence that directs expression into the periplasm was identified by comparison to the known N terminus of the protein, or, in the case of YBEJ, by homology to known leader sequences (von Heijne 1986). The protein was produced by overexpression of the processed form in the cytoplasm with an initiation methionine placed just before the N terminus of the processed protein, under the control of a strong inducible promoter in the pAED4 (Doering 1992), pET-21a (Studier et al. 1990) (Novagen), or pKK223–3 (Brosius and Holy 1984) plasmids. An oligohistidine tag was fused to the C terminus of the cloned receptor to permit facile purification by immobilized metal affinity chromatography (Hochuli et al. 1987). In all cases the receptors expressed well (at least 50 mg of pure protein per liter of fermentation). The molecular masses estimated by gel electrophoresis corresponded to the predicted mass of the expressed reading frame.

Cysteine point mutations were introduced by the PCR overlap method (Ho et al. 1989). Mutant proteins typically expressed as well as the wild-type protein. All cysteine substitutions in arabinose BP were constructed in the C64A background to prevent interference from this endogenous cysteine (Miller III et al. 1979). In the case of Fe(III) BP, all mutations were constructed in the E57D background. In the crystal structure of Fe(III) BP, this glutamate is coordinated to the iron (Bruns et al. 1997). We found that the E57D mutation weakens the affinity of Fe(III) BP for Fe(III) from approximately 1 × 10−21 M (Adhikari et al. 1995) to approximately 3 × 10−8 M, assuming a stability constant for the 1:1 Fe(III) citrate complex of logK = 10.25 (Martell and Smith 1977). This permitted straightforward determination of Fe(III) affinity by direct titration with Fe(III) citrate at nanomolar concentrations of Fe(III) BP.

Signal transduction by fluorescence

To report ligand binding by the set of 11 bPBPs, fluorescent reporter groups were attached to single cysteine thiols engineered into sites that were predicted to undergo binding-dependent conformational change. We examined eight thiol-reactive fluorophores chosen on the basis of the sensitivity of their emission spectra to changes in environment and spanning a wide range of emission and excitation wavelengths (Fig. 3). The results for all biosensor conjugates are presented in Table 5 (11 receptors, 68 cysteine mutants, 320 fluorophore conjugates).

Assessment of fluorescent biosensor function

Fluorescence emission spectra of bPBP-fluorophore conjugates were recorded in the absence and presence of saturating ligand concentrations. Spectral changes were characterized by four parameters: wavelength shift (the difference between the wavelengths of emission maximum in the unbound and ligand-saturated states), direction of intensity change (increase or decrease in intensity at the wavelengths of maximum emission in the two states), standard intensity change (ΔIstd), and standard ratiometric change (ΔR). ΔIstd is defined as the normalized intensity change relative to the average intensity, determined at the wavelength midpoint between the two emission maxima:

equation image((1))

where λstd = (λmax, unbound + λmax, saturated)/2 and I1, I2 are the fluorescence intensities at λstd of each spectrum respectively (Fig. 4A). ΔR is defined in terms of two emission bands, A1 ([λ1, λ2]) and A2 ([λ3, λ4]) (Fig. 4B):

equation image((2))

where °A1, °A2 are the areas in the absence of ligand, and A1, A2 are the areas in the presence of saturating ligand. A computer program was used to enumerate ΔR for all possible pairs of wavelength bands in the two spectra, to identify the optimal sensing condition, defined as the maximum value of ΔR. Adjustable parameters of the algorithm, and their values used for ΔRmax quantities reported here, are step size (2 nm), step width (10 nm), minimum integration area limit (fraction of total: 0.1), and maximum integration area limit (fraction of total: 1).

Analyte affinity measurements

A total of 133 bPBP-fluorophore conjugates with ΔIstd > 0.1 were used to determine ligand binding affinity by fluorimetric titration (Table 5). The emission wavelength monitored was that of maximum difference in intensity between the ligand-free and bound states. For each conjugate fluorescence intensiometric observations were fit to a hyperbolic binding isotherm for a two-state model (Marvin et al. 1997):

equation image((3))

where F is fluorescence at ligand concentration [S], Kd is the dissociation constant, and FF, FB are the fluorescence intensities of the ligand-free and ligand-saturated states, respectively. Examples of binding isotherms are shown in Figure 5 for glucose BP and glutamate/aspartate BP. For ratiometric observations, equation 33 has to be modified to account for differentially weighted contributions of the two emission bands (Lakowicz 1999):

equation image((4))

where R is ratio A1/A2, RB = A1/A2, RF = 0A1/0A2, and appKd is an apparent dissociation constant:

equation image((5))


The success of the fluorescent biosensor design strategy was evaluated by determining the probability of encountering an effectively responding fluorescent conjugate and assessing how the ligand-binding affinities are affected by the fluorophore conjugate.

Assessment of ligand-mediated changes in fluorescence

Summaries of wavelength shift, ΔIstd, and ΔRmax for all conjugates (n = 320) are presented as histograms in Figure 6A–C. The distribution of wavelength shifts was symmetrical about zero; that is, there was no overall tendency toward either blue or red shifts (Fig. 6A). Of the entire collection of conjugates, 130 show increases and 190 show decreases in fluorescence intensity upon binding. A portion of this skew is due to the finding that addition of Fe(III) citrate to all Fe(III) BP conjugates caused a decrease fluorescence emission. To examine whether this was due to quenching by Fe(III) in solution, Fe(III) citrate was added to conjugates of other bPBPs and the effect on emission intensity was monitored. It was found that Fe(III) citrate quenched fluorescence in all cases but only at concentrations much higher than those that led to the effect in Fe(III) BP. The decrease in fluorescence intensity observed in all conjugates of Fe(III) BP is therefore due to a binding-specific process and may involve relaxation of the excited state via a metal-mediated redox mechanism (Lakowicz 1999). The probability of encountering a conjugate that responds with a particular intensity declines with increasing magnitude of ΔIstd (Fig. 6B). The ratiometric response behaves similarly (Fig. 6C).

The two criteria of greatest utility for optical sensing are ΔIstd and ΔRmax. The collection of bPBP conjugates was categorized by class of steric site, fluorophore, and protein scaffold, then, for each category, quantified according to the fraction with ΔIstd > 0.25 and with ΔRmax > 1.25. The results (Tables 6 to 8, Table 7., Table 8.) give an indication of the overall success rate for finding potentially useful fluorescent biosensor conjugates. For the collection of 320 conjugates, about 24% meet the criterion for ΔIstd and about 28%, the criterion for ΔRmax.

There appears to be a correlation between signaling success rate and the sequence-related family, or cluster (Tam and Saier Jr. 1993), to which a scaffold belongs. The scaffolds having the highest success rates for ΔIstd and ΔRmax are arabinose BP, glucose BP, ribose BP, and phosphate BP (Table 6). The former three belong to cluster 2, which includes binding proteins for hexoses and pentoses, whereas phosphate BP, along with sulfate BP, belongs to cluster 6, which includes binding proteins for inorganic polyanions. The scaffolds having the lowest success rate were dipeptide BP (cluster 5, peptide and nickel binding) and the cluster 3 (polar amino acid binding) proteins glutamine BP, histidine BP, and Glu/Asp BP.

Among the three classes of attachment sites the endosteric and allosteric sites have a higher chance of meeting the threshold criteria than peristeric sites (Table 7). Success rates in terms of ΔIstd varied according to the environmental sensitivity of the fluorophore, being highest with the styryl and naphthyl dyes JPW4039, JPW4042, and JPW4045. Similarly, higher success rates for ΔRmax were associated with JPW4045 and acrylodan (Table 8).

Assessment of changes in ligand-binding affinities

The range of dissociation constants, Kd, extracted from the binding curves for each ligand is shown in Table 9. Because there is a thermodynamic linkage between ligand binding and the interaction of the attached fluorophore with the protein, the fluorophore is expected to change the intrinsic ligand dissociation constant. The change in affinity imparted by the flourophore is expected to be dependent on its location in the protein. The various conjugates exhibit a wide range of affinities (Table 9). We examined the change in affinity, defined as log(mutKd/wtKd), as a function of attachment site classification (endosteric, allosteric, or peristeric) among the 108 conjugates for which dissociation constants were measured and for which the dissociation constant of the unconjugated protein is known (Table 2). The results reveal that the three classes of site have different effects on affinity (Fig. 7). Fluorophore attachment at endosteric sites tends to perturb affinity the most, and uniformly to higher values of Kd than the wild type. Allosteric and peristeric attachment results in Kd values that are either higher or lower than the wild type, with peristeric sites exhibiting the greatest variation in effects. Interestingly, of those conjugates with higher affinity than the wild type (lower Kd), a greater proportion derives from conjugation at allosteric sites. This corroborates detailed studies in maltose BP in which affinity was increased by manipulating the volume of residues in allosteric sites (Marvin and Hellinga 2001b). The differences in effects can be rationalized in terms of the likelihood that a particular conjugate will sterically interfere either directly with ligand binding (endosteric sites, and some peristeric sites), or by influencing the intrinsic equilibrium between the open and closed states (allosteric sites, peristeric sites).

The effect on dissociation constants is determined not only by the attachment site but also by the nature of the attached fluorophore, as illustrated for arabinose BP. Dissociation constants for arabinose of the five cysteine-substitution mutants (all with the C64A mutation), measured by tryptophan fluorescence, are 5.0 μM (F23C), 3.2 μM (L253C), 3.4 μM (D257C), 7.6 μM (L298C), and 1.6 μM (K301C). Thus, the cysteine substitutions slightly perturbed affinity for arabinose (Kd of C64A mutant: 2.2 μM). The largest dependence on the attached fluorophore was found for the L253C mutant, for which Kd values ranged from 0.7 μM (acrylodan) to 775 μM (NBD). Similarly, the K394C mutant of dipeptide BP has affinities for Gly–Leu dipeptide ranging from 6 nM (NBD) to 93 μM (fluorescein). Most mutants did not exhibit such a wide range of fluorophore-dependent ligand affinity. For example, five different fluorophores conjugated to ribose BP E192C have affinities for ribose ranging from 2.6 μM (NBD and JPW4039) to 15 μM (JPW4045).

Construction of a novel biosensor using sequence information

To demonstrate that designs are not limited to those bPBPs with known structure, we introduced cysteine mutations into a paralog predicted to code for a glutamate/aspartate BP, using histidine and glutamine BPs as the structures to guide locations for likely peristeric and allosteric sites. All of the 10 sites that were tried yielded conjugates that exhibited glutamate- and aspartate-dependent changes in fluorescence. Several sites yielded good or excellent intensiometric or ratiometric sensors. Table 10 shows that the response is specific for both aspartate and glutamate, with 50- to 500-fold weaker affinity for glutamine and asparagine. Other amino acids and sugars did not elicit ligand-mediated changes in fluorescence (not shown).

Bioinformatics offers the promise of discovering new biochemical applications without direct experimentation. In the case of biosensors, individual bacterial genomes may encode scores of bPBPs that bind specific molecules to initiate transport or signal transduction (Blattner et al. 1997; Quentin et al. 1999). Few of these have been characterized, leaving a vast number untapped as scaffolds for potential biosensors. We have demonstrated the feasibility of applying genomic information, combined with structural information from homologous proteins, to construct a biosensor of novel specificity.

Previously, a glutamate/aspartate BP had been purified from E. coli (Barash and Halpern 1975; Willis and Furlong 1975) and characterized. Several pieces of evidence suggest that YBEJ corresponds to this protein. First, glutamate/aspartate BP was isolated from periplasmic extracts, consistent with ybeJ encoding a protein with a putative periplasmic localization signal sequence. Second, the previously determined molecular mass of glutamate/aspartate BP of 32 kD (Barash and Halpern 1975) or 31 kD (Willis and Furlong 1975) matches the mass of 32.5 kD predicted for the processed ybeJ product and the mass of 30 kD found by gel electrophoresis in this study. Third, the amino acid compositions determined previously (Barash and Halpern 1975; Willis and Furlong 1975) are similar to that predicted from the gene sequence, with some deviations likely attributable to inherent inaccuracy in analysis of protein acid hydrolyzates. Finally, the reported Kd values for glutamate (0.8 μM) and aspartate (1.2 μM), as well as the relatively lower affinity for glutamine and asparagine (Willis and Furlong 1975), are similar to those determined here and comparable to the Q123C-fluorescein conjugate (Table 10). Hence, ybeJ likely encodes the glutamate/aspartate BP characterized previously.

Effective sensor designs

The utility of a conjugate is determined by the absolute change in signal intensity, the ratiometric change, and the operating concentration range over which the sensor can respond accurately. Of the two observable parameters, ratiometric change is preferable to absolute intensities, because it is independent of probe concentration.

Although we define usable conjugates as having ΔIstd > 0.25 and ΔRmax > 1.25, “excellent” sensors are defined as having ΔIstd > 0.9 and ΔRmax > 2.5. The magnitudes of the changes in the excellent sensors are likely to be sufficiently large to permit robust measurements in “real-world” applications in complex fluids such as blood. Based on these criteria there are only 13 excellent absolute intensity-based sensors (4% of total), but 36 excellent ratiometric sensors (11% of total); there are 7 conjugates that are both excellent absolute intensity and excellent ratiometric sensors (Table 5). With the exception of dipeptide BP, Fe(III) BP, and histidine BP, all of the proteins have at least one excellent ratiometric and intensity-based conjugate. Glucose BP has the largest number of excellent conjugates. These conjugates all involve fluorophores known to be particularly environmentally sensitive (acrylodan, NBD, pyrene, and the styryl dyes). The incidence of excellent sensors is evenly distributed between allosteric and peristeric sites. All endosteric sites give rise to excellent sensors.

The dissociation constant of a conjugate determines the operating concentration range over which the sensor can respond accurately. The operating range guaranteed to give <5% error spans concentrations that fall within fivefold of the Kd value (Marvin et al. 1997). If the range required for accurate determination is wider than that span, then a composite biosensor can be constructed using receptors of varying affinities, as has been demonstrated for maltose BP (Marvin et al. 1997). There are three factors affecting the dissociation constant: the nature of the conjugate; the choice of emission bands for a ratiometric sensor (equation 22); and additional mutations. For particular applications these three factors can be manipulated to construct an appropriate sensor. In the next sections we describe how some of the conjugates might be deployed in real-world applications.

Glucose sensor

Among the analytes applicable to clinical medicine, glucose is one of the most important, particularly with regard to diagnosing and treating diabetes. The normal range of glucose concentration in adult human serum is 4 mM–6 mM (Burtis and Ashwood 1994). The acrylodan conjugate of the endosteric site W183C in glucose BP has an excellent ratiometric response (ΔRmax = 5.57) and a dissociation constant of 5.98 mM and is, therefore, a good candidate for detecting glucose fluctuations in the physiological range by ratiometry (Fig. 8A). Furthermore, by adjusting the ratiometric parameters, the observation window is easily extended from 5.0 to 17.4 mM, allowing all clinically relevant ranges to be observed with one sensor (Fig. 8A).

Other sensors for clinical chemistry

Amino acids are also commonly assayed in clinical tests as indicators of disease states. Histidine is an indicator of histidase deficiency (Taylor et al. 1991). The best signaling histidine BP conjugate, V163C-JPW4042, has a Kd of 0.25 μM, below the normal range in serum of about 48–125 μM. However, with sample dilution this conjugate could function effectively. Alternatively, the Kd can be adjusted by mutagenesis as was done for maltose BP (Marvin and Hellinga 2001b) and Fe(III) BP with the E57D mutation. The neuro-excitatory amino acid glutamate has normal serum concentrations of 20–220 μM (Burtis and Ashwood 1994). The best-suited biosensor is glutamate/aspartate BP F126C-acrylodan, which has a Kd of 80 μM and ΔRmax of 2.70. Glutamine is often measured in cerebrospinal fluid (Smith and Forman 1994), in which its normal range is 120–360 μM, considerably higher than the Kd (1.4 μM) of the best-signaling glutamine BP conjugate, Y163C-acrylodan. This biosensor could be used for such a purpose by mutagenesis to adjust the Kd, or by sample dilution.

Phosphate concentrations in serum and urine are clinically relevant (Burkhardt et al. 1979). Several phosphate BP conjugates signal well, the best being S39C-JPW4045, and their Kd values are all <2 μM. Inorganic phosphate in serum is typically 1–3 mM (Burtis and Ashwood 1994), requiring adjustment of the Kd or sample dilution for accurate measurements with these sensors.

Maltose concentration is relevant to a deficiency in acid maltase, with the normal plasma concentration about 2 μM (Rozaklis et al. 2002). The best maltose sensors in the present work are maltose BP conjugates S233C-JPW4042 (ΔRmax 4.0) and S233C-JPW4045 (ΔRmax 3.9), both with similar affinities (Kd ∼400 μM). Fluorescent conjugates of maltose BP mutants having affinities in the 2 μM range have been described (Marvin et al. 1997).

Industrial and environmental applications

Several bPBP conjugates may function as sensors for industrial and environmental analytes. Arabinose is relevant to improving the efficiency of ethanol production from corn (Deanda et al. 1996). Of the arabinose BP conjugates, the best signalers are K301C-NBD (Kd 31 μM, ΔRmax 3.2) and L253C-fluorescein (Kd 48 μM, ΔRmax 2.7). Ribose concentration, assayed in foods and beverages (AOAC 1995), could be measured by ribose BP conjugates T135C-acrylodan (Kd 0.4 mM, ΔRmax 6.3) and A234C-JPW4045 (Kd 3.8 μM, ΔRmax 4.1). Ratiometric sensing of ribose using a single ribose BP derivative is illustrated by the T135C-acrylodan conjugate (Fig. 8B). By varying emission wavelength bands in the fluorescence ratio (equations 4 and 54, 5), the appKd for ribose can be adjusted over a range from 41 to 146 μM (Fig. 8B). Sulfate concentrations in drinking water are of concern (EPA 1999) and could be analyzed by sulfate BP conjugate R134C-acrylodan (Kd 4 μM, ΔRmax 2.3). High concentrations of phosphate are environmentally deleterious and could be monitored using phosphate BP conjugates, as noted above for clinical applications. Iron concentration limits primary productivity in certain regions of the oceans (Martin 1992). Available ferric ion might be determined using a biosensor derived from Fe(III) BP, such as conjugate E203C-acrylodan (Kd 138 μM, ΔIstd 0.4).


We have demonstrated that it is possible to construct a large number of diverse sensors using the bPBP superfamily by coupling ligand-mediated hinge-bending motions to changes in fluorescence intensity of conjugated fluorophores by applying relatively straightforward structural design principles. Furthermore, we have shown that the approach is sufficiently robust to construct sensors using homologs whose structure is not known by applying structural homology arguments to position the fluorophores within the sequence. Fluorescent conjugates can be isolated that show large ligand-mediated changes in fluorescence and that respond in the relevant concentration range of various analytes (e.g., glucose).

Although a substantial fraction of conjugates in most bPBPs show large changes in fluorescence emission spectra, many conjugates do not. Within a given bPBP some attachment sites are more effective than others, and within a given attachment site some fluorophores are more effective than others. This points to a need to understand detailed interactions between protein and fluorophore in both the open and closed states. Studies of fluorescence quenching in NBD-conjugated glucose BP (Marvin and Hellinga 1998) showed the absence of large differences in solvent accessibility of the fluorophore between the open and closed states. In NBD-conjgated maltose BP (Gilardi et al. 1997), ligand binding induced differences in spectral properties have been interpreted in terms of altered conformations of the fluorophore. The crystal structure of a fluorophore-conjugate of phosphate BP in the ligand-bound state has been determined and used to rationalize differences in spectral properties in terms of changes in fluorophore mobility attending protein conformational change (Hirshberg et al. 1998). The challenge for future design approaches will be to generate detailed structural models of the fluorophore conjugates to predict sites and choice of fluorophore that optimize physical signal transduction.

Materials and methods

Molecular cloning

PCR was used to amplify wild-type genes for bPBPs from genomic DNA of E. coli strain CSH100 (arabinose, dipeptide, histidine, ribose, sulfate, and glutamate/aspartate BP), strain W1485 (glucose and glutamine BP) and strain RU1012 (phosphate BP), or H. influenzae strain Rd [Fe(III) BP]. Amplified products were cloned into one of the protein expression vectors pAED4 (Doering 1992), pKK223–3 (Brosius and Holy 1984), or pET vectors (Studier et al. 1990) (Novagen). N-terminal oligonucleotide primers were designed to clone only the processed periplasmic form, deleting the signal sequence. The C-terminal primer was designed to append the sequence Gly-Ser-Gly-(His)n or Gly-Ser-(His)n, where n = 5, 6, or 10. Two tandem stop codons (TAATGA) follow the last His codon. Maltose BP mutants were made in and expressed from plasmid pMAL-c2X (New England BioLabs). E. coli strains XL1-BLUE (Stratagene) and DH5α (Hanahan 1983) were used for plasmid construction. Single amino acid substitutions were generated by overlapping PCR mutagenesis (Ho et al. 1989). All clones and mutations were confirmed by nucleotide sequencing. In the case of arabinose BP the single cysteine in the wild-type sequence was replaced by alanine to eliminate the possibility of reporter group conjugation to this thiol (Miller III et al. 1979). Additionally, the sequence of Fe(III) BP was mutated by substitution of Glu57 with Asp to raise the Kd to a concentration range conveniently measured using Fe(III) citrate.

Protein expression

Plasmids were transformed into E. coli strain BL21-DE3, grown in nutrient broth overnight at 37°C, then diluted 100-fold into fresh medium and grown further at 37°C or 25°C. Expression was induced by the addition of isopropyl β-D-1-thiogalactopyranoside to 1 mM when the optical density of the culture at 600 nm reached 0.4. After 2–4 h, cells were harvested by centrifugation, resuspended in 20 mM 3-morpholinopropanesulfonic acid (MOPS), 100 mM NaCl at pH 6.9, and stored frozen or lysed immediately for protein purification.

Protein purification

Cells were lysed by sonication or by passage through a French pressure cell. The lysate was treated by adding Polymin P to 0.33% (w/v), chilling on ice for 15 min, then centrifuging to pellet cell debris. The supernatant was loaded on a Ni(II)-charged column of Chelating Sepharose Fast Flow (Amersham Pharmacia Biotech) equilibrated with 20 mM MOPS, 500 mM NaCl, 10 mM imidazole at pH 7.5. The column was washed with loading buffer, then with the same containing 60 mM imidazole, followed by the same with 100 mM imidazole. Finally, protein was eluted with loading buffer containing 400 mM imidazole and was collected in fractions and assessed for purity by gel electrophoresis. All preparations were at least 95% pure by this criterion. Protein-containing fractions were dialyzed exhaustively against buffer (20 mM MOPS, 100 mM NaCl at pH 6.9, or 20 mM NaH2PO4, 100 mM NaCl at pH 6.9) or desalted by gel filtration to remove bound ligand.

Fluorophore conjugation to cysteine-substituted bPBPs

Thiol-reactive fluorophores obtained from Molecular Probes (Eugene, OR) were 5-iodoacetamidofluorescein (fluorescein); N-(1-pyrene) iodoacetamide (pyrene); N,N'-dimethyl-N-(iodoacetyl)N'-(7-nitrobenz-2-oxa-1,3-diazol-4-yl)ethylenediamide (NBD); N-((2–(iodoacetoxy)ethyl)-N-methyl)amino-7-nitrobenz-2-oxa-1,3-diazole (NBDE); and 6-acryloyl-2-dimethylaminonaphthalene (acrylodan). The styryl and naphthyl dyes JPW4039, JPW4042, and JPW4045 (Fig. 3) were synthesized at the University of Connecticut. All fluorophore conjugation steps were typically carried out at room temperature. To protein at a concentration of 100 μM was added tris-(2-carboxyethyl)phosphine HCl to a fivefold molar excess to reduce intermolecular disulfide bonds. A thiol-reactive fluorophore (20–25 mM in acetonitrile or dimethyl sulfoxide) was added in small aliquots to a fivefold molar excess over protein. Conjugation proceeded in the dark at room temperature for 4 h, or overnight at 4°C. Separation of protein from unreacted fluorophore was achieved by exhaustive dialysis or by size-exclusion chromatography. The efficiency of reporter group attachment was assessed by determination of unreacted thiol with Ellman's reagent (Ellman 1958) or by measuring the ratio of fluorophore to protein from absorbance spectra of the purified conjugate.

Depletion of sulfate and phosphate

Solutions of sulfate BP and phosphate BP and their buffers were treated to decrease the concentration of contaminating sulfate and phosphate, respectively. Sulfate BP buffer (20 mM Tris-HCl, pH 8.0) was passed through the chloride form of Dowex 1X2–100 strongly basic anion-exchange resin. Sulfate BP solutions were treated by dialysis against treated buffer; Dowex resin held in a separate dialysis tube was also included. Phosphate BP solutions and buffer (20 mM MOPS, 100 mM NaCl at pH 6.9) were depleted of phosphate by addition of 7-methylguanosine to 1 mM and dialyzed against bacterial nucleoside phosphorylase (1 unit/mL) (Sigma-Aldrich) partitioned in a separate dialysis tube (Brune et al. 1994).


All measurements were conducted with an SLM Aminco-Bowman series 2 fluorimeter, with sample stirring at 25°C. Fluorescence emission spectra were acquired with excitation and emission slit widths of 4 and 8 nm, respectively. Photomultiplier tube potential was maintained between 400 and 800 volts. Protein concentrations were in the range of 50 to 1000 nM. Fluorophore-specific excitation was at the following approximate wavelengths: tryptophan, 290 nm; acrylodan, 390 nm; fluorescein, 485 nm; pyrene, 340 nm; NBD and NBDE, 490 nm; JPW4039, 485 nm; JPW4042, 470 nm; JPW4045, 470 nm.

To measure ligand binding affinity, ligand was serially added to 3 mL of bPBP at a concentration of 50–1000 nM, and emission intensities were recorded. Corrections were made for dilution of the protein and for background signal from buffer. Binding curves were fit to binding isotherms using equation 3 or 44, 5, as appropriate.

Fe(III) BP has a dissociation constant for Fe(III) on the order of 10−21 M (Adhikari et al. 1995), hindering accurate fluorescence-based measurements of affinity at nanomolar protein concentrations. Hence, we used Fe(III) citrate (logK = 10.25) (Martell and Smith 1977) as the ligand in a competition assay.

Table Table 1.. Potential applications of biosensors for bPBP ligands
arabinose Deanda et al. 1996 
glucoseBurrin and Price 1985AOAC 1995 
maltoseNelson et al. 1977AOAC 1995 
ribose AOAC 1995 
glutamateBurtis and Ashwood 1994AOAC 1995 
glutamineSmith and Forman 1994  
histidineTaylor et al. 1991  
phosphateBurkhardt et al. 1979 APHA 1992
sulfate  EPA 1999
Fe(III)  Martin 1992
Table Table 2.. References and PDBa files for bPBP structures, genes, and ligand binding
 Crystal structure  
bBPBOpen formClosed formDNA sequenceLigand affinity
  • a

    aProtein Data Bank (Berman et al. 2000).

  • b

    bGenBank Accession No. U47027.

arabinose BP Quiocho and Vyas 1984 1ABEScripture et al. 1987Scripture et al. 1982; Miller III et al. 1983
dipeptide BPNickitenko et al. 1995 1DPEDunten and Mowbray 1995 1DPPAbouhamad et al. 1991Guyer et al. 1986; Smith et al. 1999
Glu/Asp BP   Barash and Halpern 1975; Willis and Furlong 1975
Fe(III) BPBruns et al. 2001 1D9VBruns et al. 1997 1MRPSanders et al. 1994Adhikari et al. 1995
glucose BP Vyas et al. 1988; Vyas et al. 1994 1GLGScholle et al. 1987Anraku 1968
histidine BP Yao et al. 1994 1HSLJoshi and Ames 1996bMiller III et al. 1983
maltose BPSharff et al. 1992 1OMPSpurlino et al. 1991; Quiocho et al. 1997 1ANFDuplay et al. 1984Schwartz et al. 1976
phosphate BPLedvina et al. 1996. 1OIBLuecke and Quiocho 1990 1IXHMagota et al. 1984Medveczky and Rosenberg 1969
glutamine BPHsiao et al. 1996 1GGGSun et al. 1998 1WDNNohno et al. 1986Weiner et al. 1971
ribose BPBjorkman and Mowbray 1998Mowbray and Cole 1992 2DRIGroarke et al. 1983Willis and Furlong 1974
sulfate BP Pflugrath and Quiocho 1985; He and Quiocho 1993 1SBPHellinga and Evans 1985Jacobson and Quiocho 1988
Table Table 3.. Fluorophore conjugation sites
ProteinMutantSteric categoryaDesign methodbProteinMutantSteric categoryaDesign methodb
  • a

    a (a) Allosteric; (e) endosteric; (p) peristeric.

  • b

    b (1) Visual inspection of the closed structure; (2) identification by automated comparison of the open and closed states; (3) structural homology; (4) sequence homology.

arabinose BPD275Ca3histidine BPE167Cp1
 F23Ca3 K229Cp1
 K301Ca3 V163Cp1
 L253Ca3 Y230Cp1
 L298Ca3 F231Cp1
dipeptide BPD450Cp1 Y88Ca3
 K394Cp1maltose BZPD95Ca2
 R141Cp1 F92Ca2
 S111Cp1 I329Ca2
 T44Cp1 S233Cp2
 W315Cp1phosphate BPA225Ca2
Glu/Asp BPA207Cp4 N223Ca2
 A210Cp4 N226Ca2
 E119Cp4 S164Cp2
 F126Ca4 S39Cp2
 F131Ca4glutamine BPN160Cp2
 F270Cp4 F221Cp2
 G211Cp4 K219Cp2
 K268Cp4 L162Cp2
 Q123Cp4 W220Cp2
 T129Ca4 Y163Cp2
Fe(III) BPE203Cp1 Y86Ca2
 K202Cp1ribose BPT135Cp2
 K85Ca1 D165Cp2
glucose BPY10Ce1 A234Ca2
 N15Cp1 L236Ca2
 E93Cp1 L265Ca2
 E149Cp1sulfate BPL65Cp1
 H152Ce1 N70Cp1
 W183Ce1 Q294Cp1
 L255Ca3 R134Cp1
 D257Ca3 W290Cp1
 V296Ca3 Y67Cp1
Table Table 4.. Ligand interactions with residues in polar amino acid binding proteins
Ligand groupascscscαNαNαCscscαCαN
  • a

    a (sc) Side chain, (αN) α-amino; (αC) α-carboxy.

glutamine BPD10F13F50G68T70R75K115T118G119D157
histidine BPD11Y14L52S70S72R77L117T120T121D161
lys/arg/orn BPD11Y14F52S70S72R77L117T120T121D161
Table Table 5.. Spectral and binding parameters of fluorophore-conjugated bPBPs
ProteinaMutantSitebFluorophoreLigandλmax, apoλmax, satΔIstdcInc/decdΔRmaxcKd (μM)Std. error
  • a

    a All mutants of arabinose BP were in the C64A background; all mutants in Fe(III) BP were in the E57D background.

  • b

    b (a) allosteric, (e) endosteric, (p) peristeric.

  • c

    c Numbers in bold meet the threshold criteria of sensor utility elaborated in the test; underlined numbers indicate excellent absolute intensity or ratiometric sensors; numbers in bold italic are excellent sensors in both parameters.

  • d

    d Inc/dec, increase (+) or decrease (−) in maximum fluorescence intensity upon ligand binding.

arabinose BPD257CaJPW4039arabinose6005960.380.92903
   Acrylodan 4954950.261.66567
   Fluorescein 5195200.
   NBD 5385440.22+1.15322
 F23CaJPW4039 5875880.930.76381
   Acrylodan 5035030.02+0.993.90.6
   Fluorescein 5195190.040.453.20.5
   NBD 5435480.380.765.00.1
 K301CaJPW4039 5825881.201.73774
   Acrylodan 4864860.101.190.460.01
   Fluorescein 5185170.41+1.06241
   NBD 5325380.083.15311
 L253CaJPW4039 5905890.831.311658
   Acrylodan 4824950.051.810.690.10
   Fluorescein 5195150.242.71483
   NBD 5395390.41+1.6677549
 L298CaJPW4039 5915910.420.65702
   Acrylodan 4995000.071.77442
   Fluorescein 5185180.020.48  
   NBD 5435390.45+0.41564
dipeptide BPD450CpJPW4039Gly-Leu6026040.200.290.910.20
   JPW4042 6666640.
   JPW4045 6636660.
   Acrylodan 5085210.06+1.64114
   Fluorescein 5205200.10+0.04  
   NBD 5455440.020.80  
 K394CpJPW4039 5925980.37+1.34302
   JPW4042 6386440.06+0.99788
   JPW4045 6316400.01+1.07  
   Acrylodan 5005000.23+0.90232
   Fluorescein 5225220.30+0.21936
   NBD 5425410.060.680.0120.005
 R141CpJPW4039 5925960.060.69  
   JPW4042 6296310.060.87  
   JPW4045 6106170.151.18  
   Acrylodan 5025010.
   Fluorescein 5225220.120.663814
   NBD 5425440.00+0.13  
 S111CpJPW4039 5975980.24+0.333414
   JPW4042 6446440.18+1.4915.81.5
   JPW4045 6346420.011.07  
   Acrylodan 4995010.11+1.614.82.3
   Fluorescein 5215210.
   NBD 5385420.01+0.18  
 T44CpJPW4039 5945960.130.33  
   JPW4042 6346350.060.30  
   JPW4045 6406360.130.82  
   Acrylodan 4995010.011.52  
   Fluorescein 5225220.050.210.640.38
   NBD 5395360.110.300.0060.005
 W315CpJPW4039 5945930.260.451.000.19
   JPW4042 6456400.050.16  
   JPW4045 6406400.140.553.21.0
   Acrylodan 5035040.080.470.130.04
   Fluorescein 5215210.020.21  
   NBD 5465460.150.370.060.02
Glu/Asp BPA207CpJPW4039glutamate5925930.050.35  
   JPW4042 6356340.201.37  
   JPW4045 6376390.151.19  
   Acrylodan 4984970.26+1.61  
   Fluorescein 5205020.120.25  
   NBD 5295420.05+2.5311911
 A210CpJPW4039 5935940.080.26  
   JPW4042 6486450.110.790.1030.054
   JPW4045 6476500.090.71  
   Acrylodan 4974960.090.40  
   Fluorescein 5225220.020.14  
   NBD 5435420.020.30  
 E119CpJPW4039 5935940.12+0.34  
   JPW4045 6496440.08+1.73  
   Acrylodan 4984970.11+0.65  
   Fluorescein 5235230.050.09  
   NBD 5445440.050.25  
 F126CaJPW4039 5965920.11+0.85  
   JPW4042 6426430.01+0.40  
   JPW4045 6546430.33+1.2790394
   Acrylodan 4954820.07+2.708213
   Fluorescein 5225190.22+1.731.71 mM0.13 mM
   NBD 5715720.03+0.79  
 F131CaJPW4039 5935970.150.370.1510.080
   JPW4042 6506430.060.68  
   JPW4045 6496420.020.48  
   Acrylodan 4874920.080.84  
   Fluorescein 5225220.050.13  
   NBD 5395410.01+0.10  
 F270CpJPW4039 5965940.010.11  
   JPW4042 6406450.08+0.14  
   JPW4045 6446470.070.69  
   Acrylodan 4904920.070.60  
   Fluorescein 5235230.040.21  
   NBD 5725710.06+0.31  
 G211CpJPW4039 5945920.01+0.12  
   JPW4042 6286310.09+0.12  
   JPW4045 6316340.06+0.36  
   Acrylodan 4934920.020.29  
   Fluorescein 5225210.030.18  
   NBD 5385380.07+0.32  
 K268CpAcrylodan 4964970.030.72  
   Fluorescein 5225220.060.18  
 Q123CpJPW4039 5925880.05+0.75  
   JPW4045 6406410.000.88  
   Acrylodan 4984950.100.40  
   Fluorescein 5245220.132.330.750.09
   NBD 5445420.01+0.53  
 T129CaJPW4039 5875840.09+0.730.0930.015
   JPW4042 6496500.060.68  
   JPW4045 6446480.050.73  
   Acrylodan 4844820.04+0.52  
   Fluorescein 5235230.020.17  
   NBD 5375380.09+0.150.0190.011
Fe(III) BPE203CpJPW4039Fe(III) citrate5995920.090.37  
   Acrylodan 5185180.410.9513821
   Fluorescein 5235220.330.1541.93.5
   NBD 5505480.310.2122131
 K202CpJPW4039 6026020.240.3619329
   Acrylodan 5055030.371.1719525
   Fluorescein 5205210.300.0919516
   NBD 5425430.230.1426036
 K85CaJPW4039 5935910.050.10  
   JPW4042 6386410.030.28  
   Acrylodan 5035010.050.41  
   Fluorescein 5195200.010.03  
   NBD 5455430.080.12  
 V287CaJPW4039 5965950.130.59  
   JPW4042 5965910.060.24  
   Acrylodan 5045060.210.3422135
   Fluorescein 5215200.210.0592.57.5
   NBD 5515520.050.110.660.27
glucose BPD257CaAcrylodanglucose5055090.181.970.300.02
   Fluorescein 5235220.07+0.41  
   NBD 5455470.720.681.390.01
   Pyrene 4014020.06+0.98  
 E149CpAcrylodan 5255190.60+2.260.900.03
   Fluorescein 5275180.32+3.632532
   NBD 5495391.74+2.462.940.12
   Pyrene 3853880.81+2.6020.20.3
 E93CpAcrylodan 4614620.442.818.740.08
   Fluorescein 5235210.10+0.560.770.03
   NBD 5575460.53+3.2712.30.2
   Pyrene 3843850.11+0.82  
 H152CeAcrylodan 5275240.51+2.9748.10.5
   Fluorescein 5255190.40+2.6833.70.5
   NBD 5465491.29+1.201341
   Pyrene 4083891.75+4.6379.30.4
 L255CaAcrylodan 5065090.571.980.4940.004
   Fluorescein 5255230.23+1.490.1590.009
   NBD 5415480.19+1.710.2630.021
   Pyrene 3873850.90+0.620.1330.022
 N15CeAcrylodan 5225240.180.680.210.01
   Fluorescein 5215220.02+0.07  
   NBD 5445470.040.820.1350.007
   Pyrene 4004080.51+2.62  
 V296CaAcrylodan 5015030.000.63  
   Fluorescein 5225220.080.220.2160.006
   NBD 5415430.401.060.1690.011
   Pyrene 3883920.14+3.40  
 W183CeAcrylodan 4835040.735.575.98 mM0.03 mM
   Fluorescein 5255210.10+1.1617.6 mM2.4 mM
   NBD 5475460.130.14318 mM15 mM
   Pyrene 3913900.060.95  
 Y10CeAcrylodan 4984970.151.161163
   Fluorescein 5215210.43+1.223.31 mM0.06 mM
   NBD 5405450.03+1.28  
   Pyrene 3883910.192.87  
histidine BPE167CpAcrylodanhistidine5045060.17+0.720.0600.003
   Fluorescein 5175180.080.40  
   NBD 5395410.05+0.42  
   Pyrene 3843840.21+1.13  
 K229CpAcrylodan 5265270.020.41  
   Fluorescein 5175160.030.05  
   NBD 5325360.12+0.31  
   Pyrene 3843840.16+0.73  
 V163CpJPW4042 6596540.822.440.250.02
   Acrylodan 4935000.03+2.050.400.01
   Fluorescein 5205210.120.10  
   NBD 5425430.17+1.322.370.15
   Pyrene 3843840.08+0.78  
 Y230CpAcrylodan 5235220.020.18  
   Fluorescein 5175170.050.07  
   NBD 5355340.09+0.20  
   Pyrene 3843840.22+0.75  
 F231CpAcrylodan 5245250.010.56  
   Fluorescein 5165160.03+0.06  
   NBD 5455420.07+0.19  
 Y88CaAcrylodan 4914930.030.30  
   Fluorescein 5185180.040.06  
   NBD 5325320.010.18  
   Pyrene 3843840.15+0.44  
maltose BPD95CaJPW4039maltose5915930.080.70  
   JPW4042 6636610.010.15  
   JPW4045 6506450.08+1.360.300.01
   Acrylodan 5225010.043.31  
 F92CaJPW4039 5775830.431.74  
   JPW4042 6466460.040.11  
   Acrylodan 4954840.16+2.09  
   Fluorescein 5195180.02+0.03  
   NBD 5315330.09+0.27  
 I329CaJPW4039 5955940.050.43  
   JPW4042 6606600.05+0.60  
   JPW4045 6526490.04+0.55  
   Acrylodan 4985000.020.79  
   Fluorescein 5175180.04+0.08  
   NBD 5225230.37+1.330.200.02
 S233CpJPW4039 5775830.421.731456
   JPW4042 6706520.874.0038216
   JPW4045 6786570.42+3.9240922
   Acrylodan 5185190.010.80  
   Fluorescein 5195190.17+0.10  
   NBD 5445440.76+0.369.30.3
phosphate BPA225CaJPW4039phosphate5916010.36+2.860.0380.019
   JPW4042 6156280.301.320.390.08
   JPW4045 6216330.02+0.82  
   Acrylodan 5035020.081.95  
   Fluorescein 5225210.010.970.200.03
   NBD 5445540.811.210.270.03
 N223CaFluorescein 5195190.06+0.01  
 N226CaJPW4039 5955710.26+2.940.0660.054
   JPW4042 5736510.29+2.050.1720.148
   JPW4045 6756380.53+3.830.2770.169
 S164CpJPW4039 5995500.913.390.660.03
   JPW4042 6306150.331.781.160.22
   JPW4045 6455630.272.990.640.06
   Acrylodan 5055030.05+3.530.220.06
   Fluorescein 5215200.07+0.300.170.02
   NBD 5395400.02+0.42  
 S39CpJPW4039 5975510.363.150.420.06
   JPW4042 6236220.01+0.15  
   JPW4045 6716470.
   Acrylodan 5205200.100.80  
   Fluorescein 5195180.030.21  
   NBD 5585590.18+0.570.140.04
glutamine BPN160CpAcrylodanglutamine5295270.11+0.430.0980.023
   NBD 5465430.09+0.71  
   Pyrene 3873870.040.15  
 F221CpJPW4042 6546520.180.70  
   Acrylodan 4984980.040.40  
   Fluorescein 5185180.020.10  
   NBD 5445450.06+0.360.00990.0034
   NBDE 5385370.04+0.24  
 K219CpAcrylodan 4945000.251.340.380.03
   NBDE 5105100.02+0.21  
 L162CpAcrylodan 4965010.462.170.170.02
   Fluorescein 5235190.17+1.800.380.06
 W220CpAcrylodan 5195180.03+0.58  
   Fluorescein 5185180.010.03  
   NBD 5385380.030.45  
   NBDE 5105100.000.28  
   Pyrene 3863900.40+2.86  
 Y163CpAcrylodan 5035020.07+2.521.400.12
   Fluorescein 5185180.040.04  
   NBD 5305280.050.30  
   Pyrene 3853850.010.07  
 Y86CaJPW4042 6536530.110.830.3380.038
   Acrylodan 4904840.410.490.0520.003
   NBD 5415380.270.25  
   NBDE 5415510.12+1.81  
ribose BPA234CaJPW4039ribose5986000.371.291.840.40
   JPW4042 6686540.060.99  
   JPW4045 6365780.984.083.760.38
   Acrylodan 5045220.01+1.18  
   Fluorescein 5175170.010.05  
   NBD 5465480.28+1.630.7350.057
 D165CpJPW4039 5895930.130.36  
   JPW4042 6506520.060.27  
   JPW4045 6466470.040.77  
   Acrylodan 5015000.000.37  
   Fluorescein 5225220.030.37  
 E192CpJPW4039 5985980.440.342.570.67
   JPW4042 6466790.994.015.030.77
   JPW4045 6466660.892.4715.00.4
   Acrylodan 5165160.040.27  
   Fluorescein 5265230.12+1.3111.40.8
   NBD 5465400.00+1.672.600.26
 L236CaJPW4039 5895880.080.29  
   JPW4042 6466700.553.580.620.22
   JPW4045 6466580.251.701.530.41
   Acrylodan 5185180.090.71  
   Fluorescein 5205200.020.29  
   NBD 5185250.11+1.960.100.05
 L265CaJPW4039 6005960.010.11  
   JPW4042 6506540.912.130.260.06
   JPW4045 6696630.020.12  
   Acrylodan 5005010.200.70  
   NBD 5455400.01+0.13  
 T135CpJPW4039 6066060.020.03  
   JPW4042 6806740.02+0.35  
   JPW4045 6476640.892.45>1 mM 
   Acrylodan 5184980.31+6.260.42 mM0.01 mM
   Fluorescein 5265230.18+1.792.09 mM0.27 mM
   NBD 5425440.08+0.22  
sulfate BPL65CpJPW4042sulfate6296350.401.82  
   Acrylodan 4924820.39+2.95  
   Fluorescein 5205160.39+1.311.090.05
   NBD 5225210.020.61  
   Pyrene 3863850.13+1.20  
 N70CpJPW4042 5225220.01+0.18  
   Acrylodan 5025020.010.10  
   Fluorescein 5175170.010.01  
   NBD 5245240.010.14  
   Pyrene 3863860.010.13  
 Q294CpJPW4042 6366300.271.170.830.08
   Acrylodan 5005000.040.13  
   Fluorescein 5155140.00+0.11  
   NBD 5305300.00+0.02  
   Pyrene 3843840.01+0.08  
 R134CpJPW4039 5225180.
   JPW4042 6066080.52+0.9629.11.2
   Acrylodan 4934780.
   Fluorescein 5125120.010.020.3230.027
   NBD 5315320.580.3722.40.5
   Pyrene 3823860.15+1.30  
 W290CpJPW4042 6126240.430.890.3360.012
   Acrylodan 4964960.040.03  
   Fluorescein 5165150.04+0.09  
   NBD 5385370.060.11  
   Pyrene 3843840.16+0.37  
 Y67CpAcrylodan 5035020.000.12  
   Fluorescein 5155150.010.04  
   NBD 5365340.13+0.20  
   Pyrene 3833830.02+0.48  
Table Table 6.. Signaling parameters by binding protein
Binding proteinFraction ΔIstd > 0.25Fraction ΔRmax > 1.25n
arabinose BP0.500.4020
glucose BP0.470.5036
ribose BP0.320.4134
dipeptide BP0.080.1436
glutamine BP0.200.2425
histidine BP0.040.1324
Glu/Asp BP0.040.1554
phosphate BP0.450.5522
sulfate BP0.230.2030
maltose BP0.290.3821
Fe(III) BP0.280.0018
Table Table 7.. Signaling parameters by steric site
SiteFraction ΔIstd > 0.25Fraction ΔRmax > 1.25n
Table Table 8.. Signaling parameters by fluorophore
FluorophoreFraction ΔIstd > 0.25Fraction ΔRmax > 1.25n
Table Table 9.. Range of ligand affinities in bPBP fluorescent conjugates
bPBPLigandRange of Kd (μM)n
arabinose BParabinose0.46–77519
glucose BPglucose0.13–31800026
ribose BPribose0.1–209014
dipeptide BPGly-Leu0.006–9321
glutamine BPglutamine0.01–1.48
histidine BPhistidine0.06–2.374
Glu/Asp BPglutamate0.019–17009
phosphate BPphosphate0.038–1.212
sulfate BPsulfate0.32–298
maltose BPmaltose0.2–4096
Fe(III) BPFe(III) citrate0.66–26010
Table Table 10.. Binding specificity and affinity in mutants of glutamate/aspartate BP
  Kd (μM)
Figure Fig. 1..

Structures of 11 bPBPs, indicating locations of allo-, endo-, and peristeric sites used in this study. Each protein is shown in the closed form, with bound ligand indicated by gray ball-and-stick structures. The two domains of each bPBP are differentiated as blue or yellow ribbons, the former containing the N terminus. Hinge segments connecting the domains are green. The structure of histidine BP is used to represent the as-yet-unsolved structure of glutamate/aspartate BP. Residues mutated to cysteine are indicated by colored spheres and differentiated as allosteric (red), endosteric (orange, in GBP only), or peristeric (purple). Structures are grouped by cluster as defined by Tam and Saier Jr. (1993), according to sequence-based relationships. Cluster 2: (ABP) arabinose BP; (GBP) glucose BP; (RBP) ribose BP. Cluster 5: (DPP) dipeptide BP. Cluster 3: (QBP) glutamine BP; (HBP)histidine BP; (EBP) glutamate/aspartate BP. Cluster 6: (PBP) phosphate BP; (SBP) sulfate BP. Cluster 1: (MBP) maltose BP; (FeBP) Fe(III) BP. Molecular graphics were rendered with Molscript (Kraulis 1991).

Figure Fig. 2..

Alignment of sequences of E. coli YBEJ (putative glutamate/aspartate BP), glutamine BP, and histidine BP using clustalW (Thompson et al. 1994). Numbering begins from the putative initiation codon of the open reading frame for YBEJ, including its leader sequence. The underlined methionine is the initiation codon for expression of YBEJ used in this study. Residues in each protein that were mutated to cysteine for fluorophore conjugation are in boldface type. (a) Allosteric; (p) peristeric.

Figure Fig. 3..

Structural formulae of thiol-reactive fluorophores. Approximate wavelengths of maximal fluorescence excitation and emission, respectively, of the protein-bound fluorophores are (in nm): pyrene (340, 390); acrylodan (390, 500); fluorescein (485, 520); NBD (490, 540); NBDE (490, 530); JPW4039 (485, 590); JPW4042 (470, 640); and JPW4045 (470, 640).

Figure Fig. 4..

Definition of fluorimetric parameters. (A) Parameters λstd, I1, and I2 used to determine the standard intensity change ΔIstd. (B) Parameters A1, A2, °A, and A used to determine ΔR. Each of the areas A encompasses the respective area °A.

Figure Fig. 5..

Fluorimetric titration of glucose BP and glutamate/aspartate BP conjugates. (A) Titration of glucose BP W183C-acrylodan with glucose. (B) Titration of glutamate/aspartate BP T129C-NBD with amino acids. (•) Glutamic acid; (+) aspartic acid; (♦) asparagine; (×) glutamine. In A and B the lines shown are the best fit binding isotherms.

Figure Fig. 6..

Occurrence of fluorimetric parameters in the set of 320 fluorescent conjugates. (A) Distribution of the shift in wavelength of maximum fluorescent intensity (maxλsaturatedmaxλapo). (B) Distribution of the intensity change parameter ΔIstd. (C) Distribution of the ratiometric change parameter ΔRmax. For each parameter, the upper bound of each interval is indicated.

Figure Fig. 7..

Occurrence of changes in ligand affinity among the three classes of fluorophore attachment site. (Solid) Endosteric sites; (hatched) peristeric sites; (open) allosteric sites. In the case of arabinose BP, the value for wtKd is that of the C64A mutant, in which all conjugates were made. Data for dipeptide BP and Fe(III) BP are not included. For the former, the Kd for Gly-Leu dipeptide in the wild type has not been reported. In the case of Fe(III) BP, the Kd of the unconjugated mutant E57D was not determined. For each interval on the x-axis, the upper bound is indicated. For example, the interval labeled “0” contains values of log(mutKd/wtKd) > −1 and ≤0.

Figure Fig. 8..

Ratiometric titration of bBPB fluorophore conjugates using different pairs of emission wavelength bands. (A) Glucose BP-W183C conjugated to acrylodan, titrated with glucose at the following ratios of fluorescence emission (wavelengths in nm): (⋄) F450–459/F550–559 (appKd = 5.0 mM); (□) F450–459/F486–495 (appKd = 10.4 mM); (ø) F472–481/F450–459 (appKd = 17.4 mM). Lines show fit to equation 44. The normal serum glucose range (euglycemia) of 4 mM–6 mM is delimited by vertical lines. (B) Ribose BP-T135C conjugated to acrylodan, titrated with ribose at the following ratios of fluorescence emission (wavelengths in nm): (□) F501–510/F450–459 (appKd = 41 μM); (ø) F450–459/F501–510 (appKd = 254 μM); (⋄) F450–459/F547–556 (appKd = 461 μM).


Funding for this work was provided by grants from the National Institutes of Health and the Office of Naval Research to H.W.H. Expert technical assistance was contributed by Gregory Shirman and Sara Conrad.

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