Yusuke
Obayashi
a,
Ryota
Iino
bc and
Hiroyuki
Noji
*ad
aDepartment of Applied Chemistry, The University of Tokyo, Japan. E-mail: hnoji@appchem.t.u-tokyo.ac.jp; Fax: +81 3 5841 1872; Tel: +81 3 5841 7252
bOkazaki Institute for Integrative Bioscience, Institute of Molecular Science, National Institutes of Natural Sciences, Japan
cSOKENDAI (The Graduate University for Advanced Studies), Japan
dCREST, Japan Science and Technology Agency, Japan
First published on 1st June 2015
Digitalization of fluorogenic enzymatic assays through the use of femtoliter chamber array technology is an emerging approach to realizing highly quantitative bioassays with single-molecule sensitivity. However, only a few digital fluorogenic enzyme assays have been reported, and the variations of the digital enzyme assays are basically limited to fluorescein- and resorufin-based fluorogenic assays. This limitation hampers the realization of a multiplex digital enzyme assay such as a digital enzyme-linked immunosorbent assay (ELISA). In this study, after optimization of buffer conditions, we achieved a single-molecule digital enzyme alkaline phosphatase (ALP) assay with a cumarin-based fluorogenic substrate, 4-methylunbelliferyl phosphate (4-MUP). When ALP molecules were encapsulated in a 44-femtoliter chamber array at a low ratio of less than 1 molecule per chamber, each chamber showed a discrete fluorescence signal in an all-or-none manner, allowing the digital counting of the number of active enzyme molecules. The fraction of fluorescent chambers linearly decreased with the enzyme concentration, obeying the Poisson distribution as expected. We also demonstrated a dual-color digital enzyme assay with a ALP/4-MUP and β-galactosidase (β-gal)/resorufin-β-D-galactopyranoside combination. The activities of single ALP and β-gal molecules were clearly detected simultaneously. The method developed in this study will enable us to carry out a parallelized, multiplex digital ELISA.
In a pioneering study of a single-molecule enzyme assay in femtoliter-scaled reactors,8 a diluted solution of β-galactosidase (β-gal) was partitioned in 7–30 μm water-in-oil (W/O) droplets with a fluorescein-based fluorogenic substrate at less than 1 enzyme molecule per droplet. The fluorescence signals from the droplets exhibited an all-or-none manner; while most droplets were not fluorescent, some showed clear fluorescence. The fraction of fluorescent droplets exhibited good linearity with the enzyme concentration, indicating that partitioning of the fluorogenic assay mixture into femtoliter reactors enabled the detection of the catalytic activity of a single β-gal molecule. However, due to the large inherent heterogeneity of the W/O droplets prepared by this technique (which was developed over 50 years ago), this approach did not become widespread as an analytical method until microfabrication technology allowed generation of the femtoliter chambers with identical shapes and volumes. In 2005, Rondelez et al. first reported the digital counting of active enzyme molecules through the use of a microfabricated chamber system.6 They prepared a microfabricated PDMS sheet with identically shaped micron-sized wells on the surface and encapsulated the enzyme solution between the fabricated PDMS sheet and a glass coverslip by mechanically pressing the PDMS sheet against the glass coverslip. When the enzyme solution was diluted to a ratio of less than 1 enzyme molecule per chamber, the individual chambers showed discrete fluorescence signals in the all-or-none fashion; while most of the chambers remained non-fluorescent, a few chambers showed fluorescence, and only a few showed fluorescence signals with double intensity, indicating the encapsulation of zero, one, or two molecules in each chamber, respectively. This work demonstrated that a very simple microdevice allows the formation of identically shaped femtoliter chambers and enables the single-molecule detection of enzyme molecules and quantification of the enzyme concentrations by directly counting the number of enzyme molecules (i.e., digital counting).
In recent years, several different formats for the femtoliter chamber system have been reported. For example, researchers have reported a femtoliter chamber array system formed from a plain PDMS sheet and a chemically etched optical fiber bundle.9 In addition, Sakakihara et al. developed an array system of W/O droplets that formed on micron-sized hydrophobic patterns on glass.10 Moreover, Ge et al. integrated a droplet chamber system in a microfluidic flow channel to form a gradient of the trapping probability of target molecules along the microchannel.3 This system enables the automatic preparation of a dilution series of specimens, allowing digital counting of enzyme molecules over a wide dynamic range. A microfluidic system for the generation and analysis of freestanding femtoliter droplets was also used for digital counting of enzyme molecules.11 Recently, an arrayed lipid bilayer chamber system (ALBiC) has been developed that allows digital counting and analysis of active transporter membrane proteins.12
Recently, the application of femtoliter chamber arrays has also been expanding. For example, PDMS-based femtoliter chamber arrays have been used for measurement of the chemomechanical coupling efficiency of a single rotary molecular motor protein13 and for detection of individual translation events in single bacterial cells.14 Many reports have described other applications of femtoliter chamber array systems that provide high sensitivity and/or high-throughput capacity, including DNA sequencing,15 single-cell drug efflux activity analysis,16in vitro translation,17 and single-enzyme analysis.4,18 Among them, one of the most important applications is the digital enzyme-linked immunosorbent assay (ELISA),3,11,19,20 in which antigen molecules recognized by enzyme-conjugated antibodies are individually entrapped in a chamber, and the number of antigen molecules is counted as the number of femtoliter chambers showing enzymatically produced fluorescence signals. Although the first report of a digital ELISA used the PDMS-etched optical fiber plate system,20 droplet-based array systems have been frequently used in recent studies.3,19,21 The digital ELISA has largely improved the limit of detection (LOD) down to the femto- or attomolar range, realizing the ultrasensitivity of diagnostic ELISAs.
Compared with the active development of platforms and expansion of applications of femtoliter chamber-based digital bioassays, the variety of fluorogenic enzyme assays is still limited; however, researchers are hoping to develop parallelized digital counting assays, such as multiplex digital ELISAs, for improved analysis of multiple targets. To date, the chemistry of fluorogenic assays has mainly been based on three major fluorescent dyes: fluorescein, resorufin, and cumarin. Due to its high photostability and high fluorescent intensity, fluorescein is the first choice of probes; the first digital enzyme assay used a fluorescein derivative conjugated with galactose.6 Subsequently, digital enzyme assays with resorufin-based fluorogenic substrates were conducted for detection of β-gal,22 β-glucuronidase,4 and horseradish peroxidase.18 Although resorufin and fluorescein fluorescence signals are spectrally separable, the excitation and emission spectra overlap, causing fluorescence cross-talk. Therefore, simultaneous, dual-color digital enzyme assays using fluorescein- and resorufin-based fluorogenic assays have not been attempted. Since cumarin-based fluorogenic assays use excitation and emission wavelengths much shorter than those of fluorescein and resorufin, they will be suitable for dual digital enzyme assays with these dyes. However, digital enzyme assays using cumarin-based fluorogenic substrates have not been reported. In this study, we developed a digital enzyme assay with a cumarin-based fluorogenic substrate for detection of Escherichia coli alkaline phosphatase (ALP), which is widely used in diagnostic ELISAs.
Next, we examined the effects of diethanolamine (DEA), which enhances the transphosphorylation activity of ALP as an acceptor of inorganic phosphate.24 We also tested the effects of magnesium ions (Fig. 2B). Among the tested conditions, 1 M DEA and 1 mM MgCl2 yielded the highest ALP activity. Thus, we then tested various pH conditions with 1 M DEA and 1 mM MgCl2 (Fig. 2C). We found that pH 9.25 was the optimal pH showing the highest activity. Finally, we investigated the ALP activity at different 4-MUP concentrations to determine the basic kinetic parameters of ALP (Fig. 2D). By fitting the data points with the Michaelis–Menten equation, the maximum turnover rate (kcat) and the Michaelis–Menten constant (KM) were determined to be 1.19 × 103 s−1 and 183 μM, respectively. These values were consistent with a previous report on the mutant ALP.23
Next, digital enzyme assays for detection of the ALP activity in W/O-type femtoliter chambers were conducted at 2 mM 4-MUP in the presence of 1 M DEA and 1 mM MgCl2 at pH 9.25, at which ALP hydrolyzes 4-MUP at 1090 s−1 according to the Michaelis–Menten analysis in Fig. 2D. Note that at the estimated consumption of 4-MUP in a 44 fL chamber containing a single ALP molecule for 20 min reaction, is only 2.5%, so that the substrate consumption as well as the product inhibition would be negligible. After adding the enzyme solution to the 4-MUP solution, the reaction mixture was immediately introduced into the device and sealed with fluorinated oil. When the calculated mean number of ALP molecules per chamber (λ) was well below 1, the chambers showed a discrete fluorescent intensity. Fig. 3A shows the fluorescence image at λ = 0.52 after a 4 min incubation. Although more than 50% of the chambers remained non-fluorescent, some chambers showed weak or strong fluorescence (Fig. 3B). The fractions of non-fluorescent, weak and strong fluorescent chambers were consistent with expectations based on the Poisson distribution. When ALP molecules are randomly encapsulated, the probability of encapsulation obeys the Poisson distribution:
Next, we conducted a time-course analysis of digital enzyme assays of ALP at λ = 0.13. To minimize the photobleaching of 4-MU, images were taken every 5 min with a 100 ms exposure time (Fig. 4A). The rate of increase in fluorescence intensity was determined for each chamber by linear fitting of the time course (Fig. 4A, right). Fig. 4B shows the distribution of the rate. The leftmost peak represents the non-fluorescent chamber (0 molecule). The second peak, magnified in the inset of Fig. 4B represents the catalytic activity of a single ALP molecule at 2 mM 4-MUP. The Gaussian fit yielded an average turnover rate of 891 s−1. This value was slightly lower than the expected value from the measurement shown in Fig. 2D (1090 s−1). We do not attribute it to slow leakage of the fluorescent reaction product 4-MU into the oil phase, because the chambers enclosed with 4-MU retained almost constant fluorescence over 30 min in the control experiments (data not shown). The frequent interaction of the enzyme with surfaces might interfere with the catalysis to some extent. As expected from the Poisson distribution with λ = 0.13, a few chambers (0.7%) showed double activity by encapsulation of two enzyme molecules in a chamber (Fig. 4A and B).
In order to determine the LOD of digital counting of ALP, a 10-fold dilution series of the ALP solution from λ = 0.13 to λ = 0.00013 was subjected to digital enzyme assays. After a 10 min incubation, 120 fluorescence images of the different field of view were taken for each dilution sample. Fig. 5A shows typical fluorescence images. Each field of view contains 7600 chambers, and the total number of chambers analyzed was over 0.9 million. Because the fraction of encapsulation of two enzyme molecules in a chamber was essentially negligible at λ ≤ 0.13, each fluorescent chamber was counted as one enzyme molecule. The threshold level for fluorescent chambers was set as the mean background level plus 10 times the standard deviation (SD) of the background fluorescence. As shown in Fig. 5B, the number of fluorescent chambers was proportional to the λ and essentially consistent with the theoretical values, although the experimental values were slightly higher than the theoretical values, presumably due to the inaccuracy of protein quantification. The background count (false-positive fluorescent chambers detected in the absence of ALP) was much higher than that for the fluorogenic digital enzyme assay of β-gal with fluorescein-di-β-D-galactopyranoside (about 0.0001%).19 This difference could be explained by contaminating impurities or photoresists remaining on the device (see the Discussion section). The high background count resulted in the LOD of 7.0 fM (λ = 1.9 × 10−4) (Fig. 5C).
Finally, we tested the feasibility of dual-color digital enzyme assays of ALP and β-gal. In the fluorogenic assay for β-gal, the enzyme cleaved resorufin-β-D-galactopyranoside (RGP) to galactose and resorufin, yielding red fluorescence. The 4-MU and resorufin have different fluorescent emission peaks, 445 nm and 585 nm, respectively, and were spectrally separable in the fluorescence images. Because the optimal pH values for ALP and β-gal are different, the assays were conducted under near alkaline conditions (pH 8.25), at which ALP retains 67% of the maximum activity. After mixing well-diluted enzyme solutions with fluorogenic substrates, the reaction mixture was introduced into a flow cell and observed under a fluorescence microscope. Fig. 6 shows a pseudo-colored overlay image of 4-MU and resorufin. Green and red represent the fluorescence of 4-MU and resorufin, respectively. As expected, the green and red fluorescent chambers were distributed randomly, with some showing both green and red fluorescence (Fig. 6, yellow arrow), indicating the simultaneous encapsulation of ALP and β-gal. Thus, the feasibility of dual-color digital enzyme assays with cumarin- and resorufin-based fluorogenic assays was successfully demonstrated.
Although fluorescein- and resorufin-based digital enzyme assays have been reported independently, dual-color digital enzyme assays using these two probes have not been achieved due to overlap of their excitation and fluorescence spectra. However, cumarin emits fluorescence signals of distinctively shorter wavelengths. In this study, we verified that the dual-color digital enzyme assays for ALP and β-gal were feasible using resorufin and cumarin. Dual-color digital enzyme assays are expected to enable multiplex digital ELISAs; while such multiplex digital ELISAs have been reported using differently colored plastic beads to identify the captured antigen molecules,21 the expansion of color variations in digital enzyme assays will provide an alternative approach for multiplex digital ELISAs or further expand the multiplicity of digital ELISAs by combination with the multi-colored bead method.
In addition to the above, multi-color digital enzyme assays are expected to exhibit an improved background count compared with digital ELISAs; a high background count may impair the potential sensitivity of digital ELISAs. The main factor affecting the background count in digital ELISAs is non-specific binding of the detection antibody–enzyme conjugate to the bead surface on which the captured antibody is immobilized. Plastic beads are the most frequently used surface for antigen capture. When the target antigen molecule is marked with two different detection antibody–enzyme conjugates simultaneously, we can distinguish the true signal from the false-positive signal with high efficiency. This is because the simultaneous non-specific binding of two detection conjugates on the same bead should be much more infrequent than the single nonspecific binding events. Thus, by increasing the color variations of fluorogenic assays, the background count of digital ELISAs will be dramatically reduced. This strategy is expected to be highly effective, particularly for digital ELISAs targeting multi-epitope antigens such as infectious viruses.
However, several drawbacks of this method were also found when compared with a fluorescein-based digital enzyme assay. The first is the leakage of cumarin to the fluorinated oil phase under neutral pH conditions. Although 4-MU has an additional hydroxyl moiety on the cumarin structure which enhances water solubility, the hydroxyl group of 4-MU has to be deprotonated to prevent the leakage into the fluorinated oil phase. Actually, slow leakage was found at neutral pH (pH 7.0). This phenomenon is consistent with the pKa of the hydroxyl group of 4-MU (pH 7.8). Thus, 4-MU-based fluorogenic assays are currently limited to the conditions under which the pH is alkaline or near alkaline. Several cumarin derivatives carrying dissociative groups with different pKa values have been reported. To expand the cumarin-based fluorogenic assay to the conditions under which the pH is neutral or acidic, cumarin derivatives with lower pKa, such as a fluorinated 4-MU, should be tested.
Another drawback of cumarin-based digital enzyme assays is their relatively high background count. As shown in Fig. 5B, 0.03–0.04% of chambers showed apparent fluorescence signals under ALP-free conditions. Thus, because of this high background count, the digital counting of ALP with 4-MUP has not achieved an LOD below the fM level. We tested the possible contamination of ALP enzymes by the bacteria grown in buffers by using freshly prepared chemicals and buffers. However, the background count was not reduced. However, when observed with an optical setup for fluorescein imaging, such background counts were not observed. The background count was observed even when pure water was introduced into the device. These results suggest that the background count was attributable to the dissolution of unknown impurities from CYTOP or photoresist polymers. Thus, to reduce or eliminate the background count, microfabrication procedures may have to be improved.
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