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Analytical Chemistry
 
Anal Chem. 2016 June 21; 88(12): 6195–6198.
Published online 2016 June 1. doi:  10.1021/acs.analchem.6b01246
PMCID: PMC4917919

Monitoring Enzymatic Reactions in Real Time Using Venturi Easy Ambient Sonic-Spray Ionization Mass Spectrometry

Abstract

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We developed a technique to monitor spatially confined surface reactions with mass spectrometry under ambient conditions, without the need for voltage or organic solvents. Fused-silica capillaries immersed in an aqueous solution, positioned in close proximity to each other and the functionalized surface, created a laminar flow junction with a resulting reaction volume of ~5 pL. The setup was operated with a syringe pump, delivering reagents to the surface through a fused-silica capillary. The other fused-silica capillary was connected to a Venturi easy ambient sonic-spray ionization source, sampling the resulting analytes at a slightly higher flow rate compared to the feeding capillary. The combined effects of the inflow and outflow maintains a chemical microenvironment, where the rate of advective transport overcomes diffusion. We show proof-of-concept where acetylcholinesterase was immobilized on an organosiloxane polymer through electrostatic interactions. The hydrolysis of acetylcholine by acetylcholinesterase into choline was monitored in real-time for a range of acetylcholine concentrations, fused-silica capillary geometries, and operating flow rates. Higher reaction rates and conversion yields were observed with increasing acetylcholine concentrations, as would be expected.

There has been a recent surge in method development for studies of chemical reactions in real-time with MS. Examples include reactive desorption electrospray ionization (DESI)-MS, where reagents are delivered with an electrospray-ionization source to a reactive surface.1,2 The droplets bounce off the surface with dried down reagents and are delivered to the MS inlet for detection. Another type of setup involves mixing reagents in a syringe followed by direct infusion to the MS.37 Hence, the time-course of the reaction can be followed. Similarly, reaction kinetics of colliding droplets sprayed from two different syringes directed at each other have been studied with MS, resulting in reaction rates higher than those obtained in bulk reactions.810 However, all these techniques rely on electrospray ionization, where several kilovolts of voltage must be applied. Hence, these techniques are incompatible with studies of voltage-sensitive reactions. Also, they do not allow studies of live cells, which rapidly would get electroporated by the high voltage used in electrospray ionization.

We present a new technique, which allows for real-time interrogation of surface reactions with MS without the need for voltage. This was done by coupling a syringe pump connected to a fused-silica capillary outlet with another fused-silica capillary connected to a Venturi easy ambient sonic-spray ionization11 (V-EASI) source. V-EASI does not require voltage to generate charged droplets and relies instead on stochastically generated imbalances of droplet net charge. Further, V-EASI has successfully been used to interrogate several types of analytes, including small molecules, peptides, proteins, and nucleotides.1114 With our method, the connection of a V-EASI source to the resulting laminar flow junction was used to interrogate chemical reactions taking place on a surface deeply immersed in a liquid. The setup is conceptually similar to a continuous stirred-tank reactor (CSTR).15 However, because the setup is fully operating in the laminar flow regime and there is no active stirring, mixing with the bulk only takes place through diffusion.

Experimental Section

Chemicals

All chemicals were purchased from Sigma-Aldrich (St. Louis, MO). All solvents (MS-grade) were purchased from Thermo Fisher Scientific (Waltham, MA).

Preparation of Organosiloxane Polymer Slides

The organosiloxane polymer was prepared by stirring 500 μL of methyltrimethoxysilane and 225 μL of dimethyldimethoxysilane with 600 μL of 0.12 N acetic acid at room temperature for 30 min. Each of the 12 5 mm round wells on a Teflon-printed glass slide (Electron Microscopy Sciences, Hatfield, PA) was filled with 8 μL of reaction solution. The glass slide was kept in a covered Petri dish during the curing stage of the polymerization in a 65 °C oven for approximately 21 h. The resulting organosiloxane polymers were rinsed free of unreacted starting materials and alcohol byproduct by immersing the slides into a container of acetonitrile and agitating for 45 min. Any acetonitrile remaining on the glass slide and polymers were allowed to evaporate under ambient conditions before deposition of enzyme solution on the surface of the polymer. When not in use, the polymers were stored dry at 4 °C.

Immobilization of Acetylcholinesterase

Acetylcholinesterase was dissolved in 20 mM ammonium bicarbonate buffer, pH 7.8, to a final concentration of 2 μM. Aliquots of 10 μL were deposited on the surface of organosiloxane polymers on a glass slide and incubated overnight at room temperature (22–25 °C). The organosiloxane polymers were washed with 20 mM ammonium bicarbonate to remove any unbound acetylcholinesterase. For MS-experiments, the inflowing acetylcholine of various concentrations was also dissolved in 20 mM ammonium bicarbonate.

Real-Time Mass Spectrometry

Fused-silica tubing purchased from Polymicro Technologies (Phoenix, AZ) were used for analyte delivery and sampling. Superfusion was performed with a syringe pump (Harvard Apparatus, Holliston, MA) connected through a PEEK union (IDEX Health & Science, Rohnert Park, CA) to a fused-silica capillary. Sampling was performed with a V-EASI source made from a stainless-steel tee union (Swagelok, Solon, OH). The fused-silica capillary was fitted through the tee union and the attached 10 cm stainless-steel capillary (o.d. 1.59 mm, i.d. 0.51 mm). The fused-silica capillaries were sleeved with fluorinated ethylene propylene tubing sleeves (IDEX Health & Science, Rohnert Park, CA) to fit into the stainless-steel tee, PEEK union (IDEX Health & Science, Rohnert Park, CA) and microelectrode holders (Stoelting, Wood Dale, IL) used for fluidic connections. The microelectrode holders were operated with hydraulic micromanipulators (Narishige, East Meadow, NY), and the capillary tip positions were observed with an inverted microscope (Axiovert 135, Carl Zeiss Microscopy, Thornwood, NY). The microscope was equipped with a motorized xy-translational stage (H107, Prior Scientific, Rockland, MA) to facilitate rapid movement of the sample slide.

Mass spectrometry was performed with an LTQ-Orbitrap XL (Thermo Fisher Scientific, Waltham, MA). Mass spectra were acquired across m/z 50–500. The capillary temperature was set to 350 °C, capillary voltage was 4 kV, with maximum injection time set to 500 ms per scan for analyte sampling, operating with a N2 gas pressure at the tee inlet.

Modeling and Data Analysis

Fluid dynamics modeling was performed with COMSOL Multiphysics (COMSOL AB, Stockholm, Sweden). Data acquired with MS was analyzed with MATLAB (Mathworks, Natick, MA). Results are presented as the mean ± 1 standard deviation.

Results and Discussion

Liquid-Phase Laminar Flow Junction

The immersed tips of the fused-silica capillaries were operated with micromanipulators under a microscope where the microscopy slide holding the sample for investigation also was placed (Figure Figure11). Annotated photographs of the setup are shown in Figure S1. By applying a high gas flow in the V-EASI source, directed in parallel with the outlet of the sampling capillary, a local pressure drop caused liquid to be pulled through the capillary and delivered analytes to the inlet of the MS. We performed fluid dynamics modeling of the system, which showed that the slightly higher flow rate used for sampling (0.6 μL/min) compared to the superfusion flow rate (0.5 μL/min) was sufficient to have achieved Pe > 1 (Péclet number, defined as the ratio of advective transport rate to the diffusive transport rate). As such, a local chemical environment within the bulk solution was maintained with a volume of ~5 pL (Figure Figure22), conceptually similar to superfusion techniques used for electrophysiological cell-studies.16,17

Figure 1
Schematic view of the V-EASI MS setup used for real-time measurements of surface-reactions.
Figure 2
Fluid dynamics modeling of the liquid junction (in the absence of enzymes on the surface) where an analyte was perfused from the left side at 0.5 μL/min and collected at the right side at 0.6 μL/min. The scale bar indicates sizes within ...

Real-Time Monitoring of Hydrolysis of Acetylcholine by Acetylcholinesterase

To provide proof-of-concept of the capabilities of our system, we investigated the reaction kinetics of acetylcholinesterase, an enzyme responsible for termination of acetylcholine signaling in synaptic neurotransmission through rapid hydrolysis of acetylcholine (Scheme 1).18 Our system monitored the reaction as a function of time and provided information both about transient and steady-state conversions. In our studies, acetylcholinesterase was immobilized on an organosiloxane polymer19 through electrostatic interactions20,21 and was not removed by the relatively low salt concentration (20 mM ammonium bicarbonate) used herein. The flows of the feeding and sampling capillaries were allowed to equilibrate to achieve a steady-state concentration within the liquid junction on the glass microscope slide but outside the area that was functionalized with enzyme. With the fused-silica capillaries locked in position, the automated xy-translational stage moved the microscope slide such that the flow junction went from being in contact with the empty untreated surface to the enzyme surface in ~100 ms, traveling at 2 mm/s. To some extent, our system behaved in a similar way as a CSTR, where the apparent reaction rate is initially high and over time approaches zero; the time to reach the steady-state condition depends on the dwell time of molecules within the reaction volume and the kinetics of the reaction itself. Upon arrival at the enzyme surface, acetylcholine was rapidly hydrolyzed into choline and a steady-state was achieved within a few seconds when the feeding concentration was 1 μM acetylcholine (Figure Figure33). Representative mass spectra for times before and during exposure of the liquid junction to acetylcholinesterase are shown in Figure S2. Moving the liquid junction out of the enzyme area, levels of acetylcholine and choline returned to their initial levels. By lowering the concentration of acetylcholine, steady-state conditions took progressively longer time to achieve (Figure Figure33). Data in the range of transient kinetics (normalized to maximum intensity) were fitted with a single exponential of the form 1 – ekt (Figure S3), yielding apparent rate constants k (Table 1). In the steady-state condition, the conversion of acetylcholine into choline XACh (defined as the difference between inflow and outflow of the acetylcholine concentration at steady-state divided by the inlet concentration, using the extracted ion current as a measure of relative concentration) was progressively higher with higher substrate concentrations (Table 1).

Figure 3
Representative traces of real-time mass spectrometry monitoring conversion of acetylcholine into choline by acetylcholinesterase, surface-bound to an organosiloxane polymer. Use of a small capillary inner diameter (o.d. 150 μm, i.d. 50 μm) ...
Scheme 1
Hydrolysis of Acetylcholine by Acetylcholinesterase (AChE) Yields Choline and Acetate
Table 1
Equilibration Rates and Conversion Yields Obtained with Real-Time Mass Spectrometry for Hydrolysis of Acetylcholine with Immobilized Acetylcholinesterase (n = 3)

In conventional CSTRs with active mixing, the conversion yield can be kept constant while scaling up the volume of the system, by keeping the space time parameter τ (reaction volume-to-flow ratio) constant. In contrast, Figures Figures33 and and44 show different conversion yields during superfusion with 1 μM acetylcholine at the inlet, where XACh,50 = 0.936 ± 0.046 and XACh,200 = 0.380 ± 0.095 (p = 0.0008, Student’s t-test, n = 3), respectively, while the space time for both systems were similar (τ50 = 0.2 s and τ200 = 0.3 s), approximating the reaction volume as a half-sphere centered between the capillaries. We hypothesize the reason for this difference is that in contrast to well-mixed CSTRs, the reaction only takes place on a surface and mixing only occurs through diffusion. In Figure Figure33, the geometry of the liquid-flow junction using o.d. 150 μm, i.d. 50 μm capillaries has a larger base surface-to-volume ratio than in Figure Figure44, where o.d. 350 μm, i.d. 200 μm capillaries were used. Fluid dynamics modeling confirmed that a higher yield of conversion is to be expected (data not shown) with the experimental setup used in Figure Figure33 (qin = 0.5 μL/min, qout = 0.6 μL/min) compared to the setup used in Figure Figure44 (qin = 8 μL/min, qout = 10 μL/min).

Figure 4
Representative traces of real-time mass spectrometry monitoring conversion of acetylcholine (ACh, m/z 146.1176) into choline (Ch, m/z 104.1070) by acetylcholinesterase. Use of a large capillary inner diameter (o.d. 350 μm, i.d. 200 μm) ...

Evaluation of Optimal Operating Parameters for Real-Time Mass Spectrometry

The experimental parameters used herein were based on an evaluation of the effects of nitrogen-gas pressure, capillary geometry, and length on signal intensity using a 1 μM acetylcholine solution dissolved in 20 mM ammonium bicarbonate (Table 2). A stainless-steel capillary (o.d. 1.59 mm, i.d. 0.51 mm) was used to hold different sizes of fused-silica capillaries in the V-EASI source. Increasing pressure within the testing range and the resulting increased flow rate monotonically improved the signal intensity for fused-silica capillary with o.d. 350 μm, i.d. 75 μm. However, for the o.d. 150 μm, i.d. 50 μm capillary we found a local maximum for signal intensity at 120 psi nitrogen-gas pressure. The obtained signal intensity (mean and standard deviation obtained from data points collected over a 1 min time-course) was comparable to those resulting from the use of larger capillary sizes but operating at up to 16 times lower flow rate. These results indicated that with a sampling flow rate of 0.6 μL/min, ultimately used in this study, we could minimize sample consumption while maintaining a high signal intensity.

Table 2
Effects of Capillary Diameter, Pressure, Capillary Length, and Flow Rate on Signal Intensity and Noise

Conclusions

We have shown proof-of-concept for a novel technique which permits real-time interrogation of liquid-surface reactions with MS without the need of voltage. Several neurotransmitters and neuropeptides are nonoxidizable; hence, they cannot be directly detected with conventional amperometry. We consider that our technique may become complementary to existing techniques for live-cell measurements in future studies.

Acknowledgments

The project was supported by the National Institutes of Health, Award No. R41 GM113337 from the National Institute of General Medical Sciences and Award No. R21 DA039578 from the National Institute on Drug Abuse. E.T.J. was supported by the Swedish Research Council, through Award No. 2015-00406.

Supporting Information Available

Supporting Information Available

The Supporting Information is available free of charge on the ACS Publications website at DOI: 10.1021/acs.analchem.6b01246.

  • Description of the experimental setup, mass spectra, and an example of data fitting (PDF)

Author Contributions

Author Contributions

The manuscript was written through contributions of all authors. All authors have given approval to the final version of the manuscript.

Notes

The authors declare no competing financial interest.

Supplementary Material

References

  • Huang G.; Chen H.; Zhang X.; Cooks R. G.; Ouyang Z. Anal. Chem. 2007, 79, 8327–8332.10.1021/ac0711079 [PubMed] [Cross Ref]
  • Perry R. H.; Splendore M.; Chien A.; Davis N. K.; Zare R. N. Angew. Chem., Int. Ed. 2011, 50, 250–254.10.1002/anie.201004861 [PubMed] [Cross Ref]
  • Burkhardt T.; Letzel T.; Drewes J. E.; Grassmann J. Biochim. Biophys. Acta, Gen. Subj. 2015, 1850, 2573–2581.10.1016/j.bbagen.2015.09.016 [PubMed] [Cross Ref]
  • Lee E. D.; Mueck W.; Henion J. D.; Covey T. R. J. Am. Chem. Soc. 1989, 111, 4600–4604.10.1021/ja00195a012 [Cross Ref]
  • Dennhart N.; Letzel T. Anal. Bioanal. Chem. 2006, 386, 689–698.10.1007/s00216-006-0604-1 [PubMed] [Cross Ref]
  • van den Heuvel R. H. H.; Gato S.; Versluis C.; Gerbaux P.; Kleanthous C.; Heck A. J. R. Nucleic Acids Res. 2005, 33, e96..10.1093/nar/gni099 [PubMed] [Cross Ref]
  • Yu Z.; Chen L. C.; Mandal M. K.; Nonami H.; Erra-Balsells R.; Hiraoka K. J. Am. Soc. Mass Spectrom. 2012, 23, 728–735.10.1007/s13361-011-0323-5 [PubMed] [Cross Ref]
  • Liu P.; Zhang J.; Ferguson C. N.; Chen H.; Loo J. A. Anal. Chem. 2013, 85, 11966–11972.10.1021/ac402906d [PubMed] [Cross Ref]
  • Lee J. K.; Kim S.; Nam H. G.; Zare R. N. Proc. Natl. Acad. Sci. U. S. A. 2015, 112, 3898–3903.10.1073/pnas.1503689112 [PubMed] [Cross Ref]
  • Bain R. M.; Pulliam C. J.; Cooks R. G. Chem. Sci. 2015, 6, 397–401.10.1039/C4SC02436B [Cross Ref]
  • Santos V. G.; Regiani T.; Dias F. F. G.; Romão W.; Jara J. L. P.; Klitzke C. F.; Coelho F.; Eberlin M. N. Anal. Chem. 2011, 83, 1375–1380.10.1021/ac102765z [PubMed] [Cross Ref]
  • Antonakis M. M.; Tsirigotaki A.; Kanaki K.; Milios C. J.; Pergantis S. A. J. Am. Soc. Mass Spectrom. 2013, 24, 1250–1259.10.1007/s13361-013-0668-z [PubMed] [Cross Ref]
  • Kanaki K.; Pergantis S. A. Rapid Commun. Mass Spectrom. 2014, 28, 2661–2669.10.1002/rcm.7064 [PubMed] [Cross Ref]
  • Na N.; Shi R.; Long Z.; Lu X.; Jiang F.; Ouyang J. Talanta 2014, 128, 366–372.10.1016/j.talanta.2014.04.080 [PubMed] [Cross Ref]
  • Schmal M.. Chemical Reaction Engineering: Essentials, Exercises and Examples; CRC Press, Taylor & Francis Group:Boca Raton, FL, 2014.
  • Veselovsky N. S.; Engert F.; Lux H. D. Pfluegers Arch. 1996, 432, 351–354.10.1007/s004240050143 [PubMed] [Cross Ref]
  • Ainla A.; Jansson E. T.; Stepanyants N.; Orwar O.; Jesorka A. Anal. Chem. 2010, 82, 4529–4536.10.1021/ac100480f [PubMed] [Cross Ref]
  • Schumacher M.; Camp S.; Maulet Y.; Newton M.; MacPhee-Quigley K.; Taylor S. S.; Friedmann T.; Taylor P. Nature 1986, 319, 407–410.10.1038/319407a0 [PubMed] [Cross Ref]
  • Dulay M. T.; Eberlin L. S.; Zare R. N. Anal. Chem. 2015, 87, 12324–12330.10.1021/acs.analchem.5b03669 [PubMed] [Cross Ref]
  • Silman I.; Futerman A. H. Eur. J. Biochem. 1987, 170, 11–22.10.1111/j.1432-1033.1987.tb13662.x [PubMed] [Cross Ref]
  • Tumturk H.; Yüksekdag H. Artif. Cells, Nanomed., Biotechnol. 2016, 44, 443–447.10.3109/21691401.2014.962742 [PubMed] [Cross Ref]

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