Determination of Microbial Extracellular Enzyme Activity in Waters, Soils, and Sediments using High Throughput Microplate Assays

Summary

Microplate based procedures are described for the colorimetric or fluorometric analysis of extracellular enzyme activity. These procedures allow for the rapid assay of such activity in large numbers of environmental samples within a manageable time frame.

Abstract

Much of the nutrient cycling and carbon processing in natural environments occurs through the activity of extracellular enzymes released by microorganisms. Thus, measurement of the activity of these extracellular enzymes can give insights into the rates of ecosystem level processes, such as organic matter decomposition or nitrogen and phosphorus mineralization. Assays of extracellular enzyme activity in environmental samples typically involve exposing the samples to artificial colorimetric or fluorometric substrates and tracking the rate of substrate hydrolysis. Here we describe microplate based methods for these procedures that allow the analysis of large numbers of samples within a short time frame. Samples are allowed to react with artificial substrates within 96-well microplates or deep well microplate blocks, and enzyme activity is subsequently determined by absorption or fluorescence of the resulting end product using a typical microplate reader or fluorometer. Such high throughput procedures not only facilitate comparisons between spatially separate sites or ecosystems, but also substantially reduce the cost of such assays by reducing overall reagent volumes needed per sample.

Introduction

Microorganisms such as bacteria and fungi obtain nutrients and carbon from complex organic compounds through the production of extracellular enzymes. These enzymes typically hydrolyze polymers into smaller subunits that can be taken into the cell. Therefore, at an ecological level, these microbial extracellular enzymes are responsible for much of the nutrient mineralization and organic matter decomposition that occurs in natural environments. Enzymes such as cellobiohydrolase (CBH) and β-glucosidase are important for cellulose degradation and work in unison to catalyze the hydrolysis of cellulose to glucose^1,2, which provides a utilizable carbon substrate for microbial uptake and assimilation. The enzyme phosphatase releases soluble inorganic phosphate groups from organophosphates, essentially mineralizing phosphate and making it available for use by most organisms³. Other enzymes, such as N-acetylglucosaminidase (NAGase), are important in chitin degradation and can make both carbon and nitrogen available for microbial acquisition⁴.

One of the procedures for the assay of microbial extracellular enzyme activity in natural environments is the use of artificial p-nitrophenyl (pNP) linked substrates, an approach that was originally developed to detect soil phosphatase activity⁵. This approach relies on the detection of a colored end product, p-nitrophenol, which is released when the artificial substrate is hydrolyzed by the appropriate enzyme. The p-nitrophenol can be subsequently quantified colorimetrically by measuring its absorbance at around 400-410 nm. This method has since been applied to detect other enzymes such as NAGase⁶, and has been used in various studies looking at microbial extracellular enzyme activity in soils and sediments^7-9.

An alternative approach that was originally developed to assess extracellular glucosidase activity in aquatic environments^10,11 makes use of 4-methylumbelliferone (MUB) linked substrates. The end product released (4-methylumbelliferone) is highly fluorescent and can be detected using a fluorometer with an excitation/emission setting around 360/460 nm. A variety of MUB-linked artificial substrates are available, permitting the fluorometric measurement of the activity of at least as many enzymes (e.g. β-glucosidase, cellobiohydrolase, NAGase, phosphatase) as can be assayed using the pNP-substrate colorimetric procedure. Other microbial extracellular enzymes, such as the protein-degrading leucine aminopeptidase, can be assayed fluorometrically using 7-amino-4-methylcoumarin (COU) linked substrates. Both MUB- and COU-linked substrates have been used to determine enzyme activity in various terrestrial and aquatic samples^12,13.

While previous studies have described fluorometric or colorimetric microplate approaches to determine extracellular enzyme activity¹⁴; there is a need for a clear presentation of how to conduct such assays. Here we demonstrate procedures for conducting high throughput microplate techniques for the analysis of extracellular enzyme activity in soils and sediments using the colorimetric pNP-linked substrates approach and in natural waters using the fluorescent MUB-linked substrates technique. We focus on the measurement of the activities of β-glucosidase, NAGase, and phosphatase as these enzymes can be tied to carbon, nitrogen, and phosphorus cycling, respectively. However, the procedures described here can be applied to the measurement of other extracellular enzymes using different artificial substrates.

Protocol

Colorimetric Analysis of Extracellular Enzyme Activity in Soils and Sediments

1. Preparation of Substrate and Buffer Solutions for Colorimetric Analyses of Enzyme Activity

1. Prepare 50 mM acetate buffer (pH 5.0-5.5) by mixing 50 ml 0.1 M acetic acid (2.87 ml glacial acetic acid in 500 ml water), 150 ml 0.1 M sodium acetate, and 200 ml distilled H₂O. Adjust pH to 5.0-5.5 with 0.1 M acetic acid if necessary.
2. Prepare a solution of 1 M sodium hydroxide (NaOH) in distilled H₂O.
3. Prepare pNP-linked substrate solutions in 50 mM acetate buffer. To assay phosphatase prepare 5 mM pNP-phosphate in 50 mM acetate buffer; to assay β-glucosidase prepare 5 mM pNP-β-glucopyranoside; to assay NAGase prepare 2 mM pNP-β-N-acetylglucosaminide. Prepare all substrate solutions in sterile 15 ml or 50 ml centrifuge tubes. Solutions can be stored at 4 °C for 2-3 weeks.

2. Determination of a Standard to Convert Absorbance to pNP Concentration

1. Prepare standard solutions of p-nitrophenol in 50 mM acetate buffer. Concentrations should range from 0.025-1 mM.
2. Transfer three replicates of 100 μl of each concentration to a clear 96-well microplate. Add 10 μl 1 M NaOH and 190 μl distilled H₂O to each well.
3. Record absorbance at 410 nm using a microplate reader.
4. Multiply concentrations in the standard curve by 0.3 to get μmoles pNP per 300 μl reaction volume. Plot a curve of absorbance vs. μmole of pNP. The slope of the curve serves as the conversion factor (C) that will relate absorbance to μmole of pNP in each enzyme reaction.

3. Conducting the Enzyme Assay

1. For soil, prepare a slurry of each sample to be assayed in a sterile 15 ml centrifuge tube at a concentration of approximately 1 g/ml^-1 using 50 mM acetate buffer. For sediments, add enough acetate buffer to make the slurry easily pipettable. The exact volume of slurry needed will vary according to the number of enzymes assayed, but a minimum of 5 ml is recommended. Vortex each slurry until all clumps of soil or sediment have dispersed and note the final volume.
2. Re-vortex each slurry and immediately pipette 150 μl into each of six wells on a 96-well deepwell block (Figure 1). It is important to vortex thoroughly and frequently in order to keep soil particles in suspension. Leave at least two wells per block empty to serve as a substrate control. Note: clip the end of pipette tips with scissors prior to pipetting as soil slurries tend to clog tips. Prepare one 96-well block for each enzyme to be assayed.
3. Pour approximately 5 ml of acetate buffer into a pipette reservoir and use an 8-channel pipettor to add 150 μl of the buffer to the last two wells of each sample (these will be sample buffer controls) and the two substrate control wells (Figure 1)
4. Pour approximately 10 ml of the appropriate pNP-substrate solution into a pipette reservoir and use an 8-channel pipettor to add 150 μl of the substrate solution to the first four wells of each sample and the two substrate control wells (Figure 1). Note the time as the reaction begins as soon as the substrate solution is added.
5. Incubate plates at RT (22 °C) for 0.5-4 hr. Exact incubation time will vary depending on activity level in samples and the enzyme to be assayed. For most soils and sediments, phosphatase and β-glucosidase require incubation times of 0.5-1.5 hr, whereas NAGase and other enzymes require incubation times of >2 hr.
6. While assays are incubating prepare clear 96-well microplates to read absorbance. Prepare one microplate for each deepwell block (i.e. for each enzyme assayed). Pipette 10 μl 1 M NaOH and 190 μl of distilled water into each well of the microplate. Note: NaOH slows the enzymatic reaction and raises the pH which enhances the color of the pNP released during the reaction.
7. After incubation, centrifuge the 96-well blocks at 2,000-5,000 x g for 5 min to pellet soil particles.
8. Use a multichannel pipette to withdraw 100 μl from each well, being careful to avoid the pellet, and transfer it to the corresponding well on prepared clear 96-well microplate.
9. Turn on the microplate reader and set up any necessary software. Record absorbance at 410 nm. If the absorbance of a particular well is above the linear detection limit of the plate reader, dilute that well 1:1 with water and re-measure. If absorbance is still too high, the assay should be repeated with a shorter incubation time.

4. Determination of Dry Mass of Samples

1. Pipette 1 ml of each sample slurry into a preweighed aluminum pan.
2. Dry in a 75 °C drying oven for 48 hr and weigh. Subtract the weight of the pan from this value to obtain the dry mass of soil or sediment in 1 ml of the slurry. Multiply by a factor of 0.15 to determine the dry mass of sample in the 150 μl added to each well in the enzyme assay.

5. Calculation of Enzyme Activity per Dry Mass of Soil or Sediment

1. Calculate final absorbance of each sample by subtracting the sample control absorbance from the sample assay absorbance. If substrate controls have high absorbance (roughly >0.060) then subtract those also.
2. Calculate enzyme activity in μmoles hr^-1 g dry mass^-1 from the equation:

Enzyme activity = Final absorbance / (C x incubation time x sample dry mass)

Fluorescent Analysis of Extracellular Enzyme Activity in Natural Waters

1. Preparation of Substrate, Standard, and Buffer Solutions for Fluorometric Analyses of Enzyme Activity

1. Prepare 200 μM solutions of MUB-linked substrates (e.g. 4-MUB-β-glucopyranoside, 4-MUB-phosphate, 4-MUB-N-acetyl-β-D-glucosaminide) by dissolving the appropriate substrate in sterile (autoclaved) distilled H₂O in sterile 15 ml or 50 ml centrifuge tubes. Wrap tubes in aluminum foil to exclude light and store in refrigerator prior to use. Substrates should be stable for at least 1 week if stored in this way.
2. Prepare a MUB standard by making a stock solution of 100 μM 4-methylumbelliferone in sterile distilled H₂O. Store refrigerated in amber or foil-wrapped bottle. Immediately prior to use, dilute the 100 μM stock solution by 1/10 into sterile H₂O to make a working solution of 10 μM for enzyme assays.
3. Prepare a stock solution of 100 mM bicarbonate buffer by dissolving 8.4 g of NaHCO₃ into 1 L H₂O and autoclaving. Dilute this stock solution 1/20 into sterile H₂O as needed to make a working solution of 5 mM for enzyme assays.

2. Organizing Water Samples on a 96-Well Black Microplate

1. Organize a microplate for each enzyme following the example shown in Figure 2. Note that allowing for adequate replication, standards, and controls, this procedure can assay the activity of a single enzyme for up to nine water samples on one 96-well black microplate.
2. Pour approximately 5 ml of the first sample into a pipette reservoir and use an 8-channel pipettor to pipette200 μl into all of the wells in column 1 of the microplate(s). Discard used pipette tips and repeat as needed for each water sample to fill columns 1-9.

3. Setting up Sample, Standard, Quench, and Substrate Controls

1. Set up controls to account for samples, standards, substrate and quenching on the same black microplate as the samples (Figure 2).
2. Sample controls contain sample water and bicarbonate buffer, and are not used in the activity calculations but will demonstrate reading consistency throughout the course of the experiment. The quench controls consist of sample water and a standard amount of the fluorescent tag and are used to measure the diffraction of fluorescence in sample water. Substrate and standard controls are made up of either substrate-linked or the standard fluorescent tag, respectively, and bicarbonate buffer.
3. Pour approximately 5 ml of 5 mM bicarbonate buffer into a clean pipette reservoir. Pipette 50 μl of buffer into microplate wells 1 through 9 in Rows D and E to form two replicate wells of sample controls per sample. Change pipette tips then transfer 200 μl of bicarbonate buffer to wells 10 through 12 in Rows A and H.
4. Reduce ambient lighting by dimming or turning off lights as the fluorescent standard is light sensitive.
5. Pour approximately 5 ml of 10 μM 4-methylumbelliferone into a clean pipette reservoir. Pipette 50 μl into microplate wells 1 through 12 in Row H, and into wells 1 through 9 into Rows G and F to form three replicates of quench controls per sample and overall standard controls. Either place the microplate in the dark or cover with an opaque lid to reduce light degradation of MUB.
6. Turn on the fluorometer and set-up any necessary software to be ready to read before adding the substrate. Note: some fluorometer bulbs may require a warm-up time of 3 min or more.
7. Pour approximately 5 ml of the appropriate MUB-linked substrate (e.g. 4-MUB-phosphate) into a clean pipette reservoir. Use a 12-channel pipettor to pipette 50 μl into microplate wells 1 through 12 in Row A, and into wells 1 through 9 in Rows B and C to form three replicate assays for each sample and three substrate controls. Immediately proceed to step 4.1, recording fluorescence.

4. Recording Fluorescence

1. Read the initial fluorescence immediately after substrate addition to the microplate. After reading fluorescence, incubate the microplate at RT (22 °C) either in the dark or covered with an opaque lid to reduce light degradation of MUB.
2. The incubation time required to measure the maximum potential enzyme activity in a water sample will depend on the enzyme concentration within the sample. Since this is unknown before the assay is completed, the microplate will have to be read at multiple time steps. Typically, reading at intervals of 10-15 min over the course of 1 hr is acceptable for many enzymes, although samples with very high activity for certain enzymes may peak before 10 min.
3. Continue reading fluorescence in the microplate at your designated intervals for at least 1 hr. Be sure to keep the microplate covered or in the dark between readings.

5. Calculation of Enzyme Activity per Volume of Water

1. For each sample at each time interval calculate the: mean initial sample fluorescence (wells D and E), the mean final sample fluorescence (wells A-C), the mean standard fluorescence (wells H10-11), and the mean quench control fluorescence (wells F-G).
2. For each time interval, calculate enzyme activity in nmoles hr^-1 ml^-1 from the equation:

Enzyme activity = (mean sample fluorescence - mean initial sample fluorescence) / ((mean standard fluorescence / 0.5 mol) x (mean quench control fluorescence / mean standard fluorescence) x (0.2 ml) x (time in hr))

3. Examine the activity values calculated for each time step. Determine final potential activity from the time step with the highest activity. If activity values continue to increase then later time steps may be required; if activity values fall throughout the course of the run, then run again with shorter time steps. Final activity is in nmoles of substrate consumed hr^-1 ml^-1 but can be scaled up to express as μmoles hr^-1 L^-1.

Results

Soils and aquatic sediments typically have appreciable levels of extracellular enzyme activity as a result of attached microbial communities (biofilms) growing on the surface of particles. Figure 3 shows how this activity changes depending on the size of particles obtained from the surface sediment of a third order stream in northern Mississippi, USA. A previous study has shown that the bacterial communities on sediment particles from this stream can be separated into three distinct groups based on molec...

Discussion

Determining the activity of a variety of microbial extracellular enzymes in soils and sediments can provide useful insights into rates of nutrient mineralization and organic matter processing¹⁷. However, soils can vary in their moisture levels, so it is important to standardize activity to soil dry weight. This requires an additional drying step (typically of two days) beyond simply measuring enzyme activity. Thus, in contrast to assays of enzyme activity in water samples that provide near instantaneous result...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
REAGENTS AND MATERIALS
Glacial acetic acid			Various suppliers
Sodium acetate			Various suppliers
Sodium hydroxide			Various suppliers
p-Nitrophenol	Fisher	BP612-1	Alternates available
p-Nitrophenyl (pNP)-phosphate	Sigma	N3234	pNP-substrate
pNP-β-glucopyranoside	Sigma	N7006	pNP-substrate
pNP-β-N-acetylglucosaminide	Sigma	N9376	pNP-substrate
Clear 96-well microplates	Fisher	12-563-301	Alternates available
96-well deep well blocks	Costar	3958	Alternates available
Aluminum weigh pans			Various suppliers
Sterile 15 ml centrifuge tubes			Various suppliers
Sterile 50 ml centrifuge tubes			Various suppliers
4-Methylumbelliferone	Sigma	M1381
4-Methylumbelliferyl (MUB)-phosphate	Sigma	M8883	MUB-substrate
4-MUB-glucopyranoside	Sigma	M3633	MUB-substrate
4-MUB-N-acetylglucosaminide	Sigma	M2133	MUB-substrate
Sodium bicarbonate			Various suppliers
Black 96-well microplate	Costar	3792
Pipette reservoir			Various suppliers
EQUIPMENT
Centrifuge	Eppendorf	5810R
Centrifuge rotor	Eppendorf	A-4-81	For microplates/deep-well blocks
Microplate reader	BioTek	Synergy HT	Alternates available
Microplate fluorometer	BioTek	FLx 800	Alternates available
8-channel pipettor			Various suppliers