Activation and Conjugation of Soluble Polysaccharides using 1-Cyano-4-Dimethylaminopyridine Tetrafluoroborate (CDAP)

Andrew Lees; James Zhou

doi:10.3791/62597

JoVE Journal > Immunology and Infection

Immunologia e infezioni

Activation and Conjugation of Soluble Polysaccharides using 1-Cyano-4-Dimethylaminopyridine Tetrafluoroborate (CDAP)

Published: June 14, 2021

doi:

10.3791/62597

Andrew Lees¹, James Zhou¹

¹Fina Biosolutions LLC

Summary

Proteins and amine-containing ligands can be covalently linked to polysaccharides activated by the cyanylation reagent, 1-cyano-4-dimethylaminopyridine tetrafluoroborate (CDAP), to form covalent protein (ligand)-polysaccharide conjugates. This article describes an improved protocol for carrying out controlled CDAP activation at 0 °C and varying pH and performing subsequent conjugation of the activated polysaccharides.

Abstract

Conjugate vaccines are remarkable advances in vaccinology. For the preparation of polysaccharide conjugate vaccines, the polysaccharides can be conveniently functionalized and linked to vaccine carrier proteins using 1-cyano-4-dimethylaminopyridine tetrafluoroborate (CDAP), an easy-to-handle cyanylating reagent. CDAP activates polysaccharides by reacting with carbohydrate hydroxyl groups at pH 7-9. The stability and reactivity of CDAP are highly pH-dependent. The pH of the reaction also decreases during activation due to the hydrolysis of CDAP, which makes good pH control the key to reproducible activation. The original CDAP activation protocol was performed at room temperature in unbuffered pH 9 solutions.

Due to the rapid reaction under this condition (<3 min) and the accompanying fast pH drop from the rapid CDAP hydrolysis, it was challenging to quickly adjust and maintain the target reaction pH in the short time frame. The improved protocol described here is performed at 0 °C, which slows CDAP hydrolysis and extends the activation time from 3 min to ~15 min. Dimethylaminopyridine (DMAP) was also used as a buffer to pre-adjust the polysaccharide solution to the target activation pH before adding the CDAP reagent. The longer reaction time, coupled with the slower CDAP hydrolysis and the use of DMAP buffer, makes it easier to maintain the activation pH for the entire duration of the activation process. The improved protocol makes the activation process less frenetic, more reproducible, and more amenable to scaling up.

Introduction

Conjugate vaccines, such as those consisting of polysaccharides covalently linked to a carrier protein, are among the remarkable advances in vaccinology¹^,². Polysaccharides, as T-cell-independent antigens, are poorly immunogenic in infants and do not induce memory, class switching, or affinity maturation of antibodies³. These shortcomings are overcome in polysaccharide conjugate vaccines⁴. As most polysaccharides do not have a convenient chemical handle for conjugation, they must first be made reactive or "activated." The activated polysaccharide is then linked either directly with the protein (or modified protein) or is functionalized for additional derivatization before conjugation⁴. Most licensed polysaccharide conjugate vaccines use either reductive amination or cyanylation to activate polysaccharide hydroxyls. Cyanogen bromide (CNBr), a reagent that had previously been used to activate chromatography resins, was initially used for polysaccharide derivatization. However, CNBr requires high pH, typically ~ pH 10.5 or greater, to partially deprotonate polysaccharide hydroxyls so that they are sufficiently nucleophilic to attack the cyano group. The high pH can be detrimental to base-labile polysaccharides, and neither CNBr nor the active cyano-ester initially formed is sufficiently stable at such high pH.

CDAP (1-cyano-4-dimethylaminopyridine tetrafluoroborate; Figure 1) was introduced by Lees et al. for use as a cyanylating agent for the activation of polysaccharides⁵^,⁶. CDAP, which is crystalline and easy to handle, was found to activate polysaccharides at a lower pH than CNBr and with fewer side reactions. Unlike CNBr, CDAP-activated polysaccharides can be directly conjugated to proteins, simplifying the synthesis process. CDAP-activated polysaccharides can be functionalized with a diamine (e.g., hexane diamine) or a dihydrazide (e.g., adipic dihydrazide, ADH) to make amino- or hydrazide-derivatized polysaccharides. A high concentration of the homobifunctional reagent is used to suppress crosslinking of polysaccharides. Amino polysaccharides can then be conjugated using any of the myriad techniques used for protein conjugation. Hydrazide-derivatized polysaccharides are often coupled to proteins using a carbodiimide reagent (e.g., 1-ethyl-3-(3-dimethylaminopropyl)carbodiimide (EDAC))⁷. Further optimization of CDAP polysaccharide activation has been described by Lees et al.⁸ and is incorporated into the protocol described here.

CDAP conjugation overview
The CDAP protocol can be conceptualized as two phases: (1) the activation of the polysaccharide and (2) conjugation of the activated polysaccharide with a protein or ligand (Figure 2). The goal of the first step is to efficiently activate the polysaccharide, while the goal of the second is to efficiently conjugate to the activated polysaccharide. The activated polysaccharide ties the two steps together. This conceptualization helps focus on the critical elements of each step. Figure 2 expands on this conceptualization, showing the desired activation and coupling reactions, along with the hydrolysis reactions and side reactions.

During the activation phase, the three major concerns are CDAP stability, CDAP reaction with the polysaccharide hydroxyls, and the stability of the activated polysaccharide (Figure 3). CDAP hydrolysis increases with pH, as does the hydrolysis of the activated polysaccharide and the side reactions. However, the CDAP reaction with the polysaccharide is facilitated by increasing the pH. Efficiently activating polysaccharides with CDAP requires a balance between 1) the reactivity of the polysaccharide and CDAP and 2) the hydrolysis and side reactions of both the reagent and the activated polysaccharide.

In the original CDAP activation protocol described by Lees et al.⁵, CDAP activation of polysaccharides was carried out at room temperature in unbuffered pH 9 solution. The rate of activation was found to be rapid under this condition, and the activation would be complete within 3 min. The reaction was also accompanied by rapid hydrolysis of CDAP, causing a rapid pH drop of the unbuffered reaction solution. It was challenging to quickly raise and to maintain the reaction pH at the target value in such a short time frame. In the described protocol, activation was performed by adding CDAP from a 100 mg/mL stock solution to the unbuffered polysaccharide solution. The pH was raised 30 s later with "an equal volume of 0.2 M triethylamine". Protein to be conjugated was then added after 2.5 min to the activation reaction. Notably, the pH of the activation step was not well controlled and most likely initially exceeded the target pH. The fast reaction requiring prompt pH adjustment made the activation process difficult to control and challenging to scale up.

In contrast to the original protocol, the modified protocol described here has two major improvements. First, the pH of the polysaccharide solution is pre-adjusted to target activation pH, using DMAP as the buffer, before the addition of CDAP. DMAP has a pKa of 9.5 and thus has good buffering power around pH 9, and unlike many other buffers, DMAP was not found to promote CDAP hydrolysis⁸. Furthermore, DMAP is already a process intermediate and therefore does not add a new component to the reaction mixture. Pre-adjusting the pH before adding CDAP eliminates the large pH swing at the beginning of the reaction and allows for more efficient maintenance of the target pH during the reaction. The second improvement is to perform the activation reaction at 0 °C, where the rate of CDAP hydrolysis is markedly slower than that at room temperature. With the longer reagent half-life at 0 °C, the activation time is increased from 3 min to 15 min to compensate for the slower activation rate at the lower temperature. The longer reaction time, in turn, makes it easier to maintain the reaction pH. The use of 0 °C also slows the degradation of pH-sensitive polysaccharides, making it possible to prepare conjugates of this type of polysaccharide. The improvements in the protocol make the activation process less frenetic, easier to control, more reproducible, and more amenable to scaling up.

This article describes the improved protocol for carrying out controlled CDAP activation of polysaccharide at 0 °C and at a specified target pH and performing subsequent derivatization of the activated polysaccharides with ADH. Also described is a trinitrobenzene sulfonic acid (TNBS) assay, based on the method of Qi et al.⁹, for the determination of hydrazide level on the modified polysaccharide. A modified assay for hexoses based on resorcinol and sulfuric acid¹⁰ is also described, which can be used for determining a broader range of polysaccharides. For more information on CDAP activation and conjugation, the reader is referred to earlier publications⁵^,⁶^,⁸ by Lees et al.

Protocol

NOTE: Prepare the polysaccharide solution, ADH solution, DMAP solution, and CDAP stock solution in advance before executing the polysaccharide activation and functionalization procedures. Place the solutions and equipment in an organized, convenient, and logical location. The reaction described is for 10 mg of polysaccharide and can be scaled up or down. It is recommended to evaluate the protocol at a small scale before scaling up.

1. Prepare 5 mg/mL polysaccharide solution, 2 mL.

For lyophilized polysaccharide
1. Allow the polysaccharide container to come to room temperature before opening. Weigh out 10 mg of polysaccharide inside a screw-cap tube using an analytical balance. Use a static eliminator for easier sampling and more accurate weighing of the powder.
2. Add 2 mL of 0.15 M sodium chloride (NaCl) to the tube to dissolve the polysaccharide. Cap and vortex the tube.
  NOTE: Sodium chloride does not affect the CDAP reaction, but it may affect the polysaccharide secondary structure. Some polysaccharides are more soluble at different salt concentrations.
3. Mix the tube by end-over-end rotation for 12-24 h, depending on the polysaccharide molecular weight, to allow the polysaccharide to hydrate fully. If necessary, gently warm the tube to promote solubilization.
For solubilized polysaccharide in buffered solution
NOTE: For efficient CDAP activation, the polysaccharide solution should not contain any buffer, especially phosphate ion. Follow the procedure below to replace the buffer with water or a saline solution and to adjust the polysaccharide concentration to 5 mg/mL.
1. Obtain a 4 mL or 15 mL centrifugal-spin filter device of the appropriate molecular weight cutoff (MWCO).
  NOTE: The MWCO is ideally 5-10 times smaller than the molecular weight of the polysaccharide.
2. Add a volume of the buffered polysaccharide solution containing ~20 mg of the polysaccharide to the filter insert. Fill to the full mark with water or a saline solution. Cap the filter tightly. Mix by end-over-end a few times.
3. Centrifuge the filter device at the centrifugal force suggested by the manufacturer. Ensure that the centrifugation time is long enough to achieve at least 5-fold volume reduction after each spin. Discard the flow-through. Reassemble the filter device.
4. Refill the filter insert to the full mark with fresh water or saline solution. Cap the filter tightly. Mix the content in the filter by end-over-end rotation ~10 times or by gentle vortexing; repeat the spin.
  NOTE: Polysaccharide can accumulate at the bottom of the filter insert of the centrifugal device, forming a gel. It is recommended to re-mix the retentant inside the filter insert with the fresh refill before the next spin.
5. Repeat the refill and spin cycle for a minimum of 3 times.
6. Follow the exercise below to recover the polysaccharide retentant from the filter insert.
  1. Add fresh water or saline to the filter insert so that the volume is ~1 mL. Mix by pipetting up and down or by gentle vortexing.
  2. Transfer all of the mixed retentant to a 5 mL tube. Add 1 mL of fresh water or saline to the filter insert. Rinse the filter by pipetting up and down or by gentle vortexing. Transfer and combine all of the rinses with the recovered polysaccharide.
7. Determine the polysaccharide concentration (see the polysaccharide assay in section 7.3). Dilute the polysaccharide with additional water or saline to 5 mg/mL.
When the polysaccharide solution is prepared, chill the tube containing the polysaccharide solution in an ice bucket.

2. Prepare 0.5 M adipic acid dihydrazide (ADH) solution, 10 mL.

Weigh 0.87 g ADH in an analytical balance, and solubilize in 8 mL of 0.1 M HEPES (4-(2-hydroxyethyl)-1-piperazineethanesulfonic acid), pH 8.
Adjust to the target pH with 1 M sodium hydroxide (NaOH), monitored by a pH meter. Bring to 10 mL with additional buffer and re-confirm the pH.

3. Prepare 2.5 M DMAP solution, 10 mL.

NOTE: DMAP is toxic and will penetrate the skin. Wear nitrile gloves when performing the procedure.

Carefully weigh 3 g of DMAP into a 50 mL conical tube. Add 5 ml of water to DMAP and mix by vortexing for 5 min to obtain a cloudy solution (~ 7 mL).
While mixing, add 50 µL increments of 10 N hydrochloric acid (HCl) to the DMAP solution. Mix between each addition. Stop adding when the solution becomes clear.
Add 10 N NaOH in 25 µL increments to bring the DMAP solution to ~pH 8.
Bring the DMAP solution to 10 mL with water to give a 2.5 M solution.
Fine-tune the pH of the 2.5 M DMAP solution.
NOTE: DMAP solution pH changes with concentration and ionic strength. This exercise is to fine-tune the 2.5 M DMAP stock to a specific pH so that when it is mixed with 10 volumes of polysaccharide, the resulting solution is close to the target pH for activation.
1. Prepare a series of 1.5 mL tubes containing 1 mL of water or the NaCl solution, whichever was used for preparing the polysaccharide solution. Chill the tubes on ice.
2. Add 100 µL of DMAP to a chilled tube. Vortex and measure the pH with a pH meter. Then, discard the measured tube.
3. If the measured pH is not close to the target value, adjust the pH of the DMAP stock with 1 M NaOH or HCl as appropriate. Repeat steps 3.5.2 and 3.5.3 until the measured pH is close to the target pH.

4. Prepare 100 mg/mL CDAP stock solution

NOTE: CDAP powder should be kept tightly closed and stored at -20 °C and allowed to come to room temperature before opening. Wear nitrile gloves when performing the procedure.

Tare a 1.5 mL snap-cap microcentrifuge tube on an analytical balance. Using a small spatula, weigh out 10-140 mg of CDAP into the tube. Note the actual weight of CDAP.
Determine the volume of acetonitrile needed to prepare 100 mg/mL CDAP. Open acetonitrile in a fume hood.
Using an appropriate volume pipet, draw and release the acetonitrile to equilibrate its vapor in the pipet tip. Wait for the solvent to drip out of the pipet tip after a few seconds, and be prepared to transfer it to the CDAP tube directly. Draw the calculated volume of acetonitrile and directly transfer it to the CDAP tube. Snap the cap shut.
NOTE: Acetonitrile can also be transferred to the CDAP tube using a Hamilton syringe or its equivalent of suitable size.
Vortex to fully solubilize the CDAP. Place the CDAP tube in an ice bucket.
NOTE: CDAP is stable in acetonitrile in the cold. Soluble stocks may be kept at -20 °C for >1 week. However, it is preferable to prepare fresh CDAP solutions.

5. Polysaccharide activation and hydrazide functionalization

Ensure all of the following items are ready and solutions chilled on ice before starting the activation: 2 mL of a 5 mg/mL polysaccharide solution in a flat-bottom, wide-mouth container containing a stir bar, placed on top of a magnetic stirrer; 100 mg/mL CDAP stock solution; 2.5 M DMAP stock solution; a pH meter with a semi-micro pH probe, such as the 6 mm diameter probe, calibrated for 0 °C according to the manufacturer's instructions; a 100 µL pipet ready to use; a timer cleared and ready to use; an autotitrator dispenser head positioned or 10 µL pipet ready to use; 0.5 M ADH solution.
Pre-adjust the pH of the polysaccharide to the target pH using DMAP.
1. Place the pH probe into the polysaccharide solution and leave it in the solution during the entire activation procedure.
2. Transfer 200 µL of the DMAP stock solution to the polysaccharide solution by dropwise addition under stirring.Adjust the pH of the solution to the target activation pH. Add 0.1 M HCl to lower the pH and 0.1 M NaOH to increase the pH. Avoid exceeding the target pH by more than 0.1 pH unit, and keep the reaction chilled in an ice-water bath for the duration of the activation.
CDAP activation
1. Pipet 100 µL CDAP up and down to equilibrate the vapor in the pipet tip. Transfer 100 µL of CDAP to the polysaccharide solution with stirring.
  NOTE: This activation uses 1 mg of CDAP for 1 mg of polysaccharide as a starting ratio. The ratio can be increased or decreased when optimizing the activation.
2. Start the timer and monitor the pH change during the entire activation. Maintain the reaction at the target pH by promptly adding 10 µL increments of 0.1 M NaOH to the reaction, with the aid of an autotitrator dispenser (or pipet).
  NOTE: It may help reduce the pH response time to stir with a pH probe gently. The pH drops more rapidly in the beginning, and it may be necessary to add the 0.1 M NaOH more frequently. As the reaction proceeds, the pH decrease becomes slower, and the addition becomes less frequent. The pH should remain essentially unchanged when approaching the optimal activation time, which is 10-15 min for pH 9 activation.
ADH functionalization
1. When the optimal activation time is reached, add 2 mL of 0.5 M ADH all at once to the activated polysaccharide under stirring. Check that the pH is in the target range (pH 8-9 for ADH).
  NOTE: One addition with quick mixing minimizes the probability for both ends of the dihydrazide to react with the activated polysaccharide, preventing polysaccharide crosslinking.
2. Continue to stir the reaction mixture for at least 1 h. Transfer the reaction mixture to 4 °C, but 0-20 °C is acceptable.
  NOTE: The ADH functionalization reaction is not strongly dependent on temperature. As the large excess of dihydrazide acts as the quenching reagent, it is not necessary to further quench the activated polysaccharide. However, when directly conjugating proteins, the reaction should be quenched, typically with 1 M glycine, pH 8-9.

6. Purification of ADH-functionalized polysaccharide by dialysis

NOTE: The crude product from the ADH functionalization reaction contains a high concentration of ADH (0.5 M), which can be removed most efficiently by extensive dialysis. Gel filtration, either with a column or a spin desalting device, is not as efficient, especially when it is required to remove the residual ADH contaminant.

Determine the MWCO of the dialysis membrane. Use a 3 kDa cutoff for smaller polysaccharides.
NOTE: The MWCO of the dialysis membrane is ideally 5-10 times smaller than the MW of polysaccharide.
Choose the desired dialysis format (cassettes or tubings) and the correct device capacity. Ensure that the device capacity is 2 times larger than the sample volume. Consult the manufactures' instructions for using the device.
Hydrate the dialysis membrane in water before use. Transfer the crude derivatized polysaccharide solution to the dialysis device according to manufacturers' instructions.
NOTE: Wear nitrile gloves to avoid contact with DMAP.
Dialyze in a container filled with 2-4 L of 1 M NaCl and a stir bar. Place the container on a stir plate in a cold room or inside a refrigerator. Stir the dialysate gently and continuously during dialysis.
After dialyzing for at least 4 h, change to fresh 1 M NaCl, and dialyze for at least 12 h. Dialyze against 2 changes of 0.15 M saline, each for at least 12 h. If desired, dialyze against 2 changes of water.
Verify if all the ADH is removed by testing the overnight dialysate using a quick TNBS test.
1. Obtain 3 borosilicate tubes, label them as negative control (ctrl), positive ctrl, and sample, respectively.
2. To the negative ctrl tube, add 975 µL of 0.1 M borate, pH 9.
3. To the positive ctrl tube, add 100 µL of 0.05 mM ADH (0.1 mM hydrazide) and 875 µL of 0.1 M borate, pH 9.
4. To the sample tube, add 500 µL of the overnight dialysate and 475 µL of 0.1 M borate, pH 9.
5. Add 25 µL of 1% TNBS to all three tubes. Mix well. Place in the dark for 1 h.
6. Compare the color intensity of the 3 tubes in 1 h. Ensure that the sample tube color intensity is in-between that of the positive ctrl and the negative ctrl, which indicates that the ADH contaminant is down to 0.01 mM or below. Dialyze one more time.
  NOTE: It is prudent to reduce the level of the ADH contaminant as much as possible so that the ADH hydrazide accounts for less than 1% of the total hydrazide in the purified hydrazide-polysaccharide.
7. Recover the derivatized polysaccharide from dialysis. Determine the concentration of the polysaccharides and hydrazide. Calculate the hydrazide/polysaccharide ratio (see section 7). If the dialyzed polysaccharide must be concentrated to 5-10 mg/mL, consult section 1.2.

7. Analysis of hydrazide-derivatized polysaccharides

NOTE: The purpose of the analysis described here is to determine the polysaccharide concentration, the hydrazide concentration, and the level of hydrazide derivatization in terms of the hydrazide/polysaccharide ratio.

Sample preparation
NOTE: Polysaccharides to be assayed need to be free of low molecular weight carbohydrate, amine, or hydrazide impurities. Lyophilized samples should be dry and salt-free to ensure accurate weight measurement. Usually, ~1 mL of a 1-2 mg/mL solution is adequate for assays.
1. Weigh at least 10 mg of the lyophilized polysaccharide sample on an analytical balance, using a non-static spatula or a static eliminator. Dissolve the polysaccharide in water or saline to a concentration (e.g., 2 mg/mL) so that the assay signals fall within the linear range of the standard curve.
2. Mix end-over-end and allow enough time for the sample to dissolve completely. Perform overnight hydration depending on polysaccharide molecular weight.
Polysaccharide assay: resorcinol/sulfuric acid method
NOTE: The appropriate assay for polysaccharides will depend on the carbohydrate composition of the polymers. The original resorcinol/sulfuric acid assay was intended for hexose sugars¹⁰. The assay was modified here by raising the temperature of the heating step from 90 °C to 140 °C. At this higher temperature, the assay loses some specificity but can be used to assay many sugars. However, it is still necessary to determine the suitability of the assay for a particular polysaccharide. Triplicates are recommended for each point, but some accommodation may be necessary due to the capacity of the heating block.
1. Prepare 75% sulfuric acid
  NOTE: Concentrated sulfuric acid is extremely corrosive and can cause severe burns. Perform this procedure in a chemical fume hood. Always pour concentrated acid into water, not vice versa!
  1. Add 50 mL of water to a 200 mL glass bottle. Place the bottle in a cold water bath. Slowly add 150 mL of sulfuric acid. Cap the bottle so that it is vented.
  2. Allow the solution to equilibrate to room temperature. Use the solution within 3 months.
2. Prepare carbohydrate standards
  1. Prepare the unmodified polysaccharide solution at 1 mg/mL to be used as the standard. Alternatively, use a mix of individual sugars in the ratio found in the repeat unit of the polysaccharide, at 1 mg/mL of the total sugar concentration, as the standard.
    NOTE: Although the sugar mix will usually give the same result as the carbohydrate polymer of identical sugar composition, this should be confirmed experimentally.
3. Ensure that the heating block with tube holders for 13 x 100 borosilicate test tubes is functioning. Use a protective pad underneath and surrounding the heating block in case of acid spills. Pre-heat the heating block to 140 °C for a minimum of 1 h to achieve stable, uniform temperature through all the blocks utilized.
4. Label 13 x 100 borosilicate test tubes, triplicate for each standard and each sample. Add 0, 2.5, 5, 7.5, 10 µg (or µL) of the 1 mg/mL carbohydrate standard to the correspondingly labeled standard tubes. Add water to each tube to bring the volume to 100 µL.
  NOTE: The color generated is dependent on specific sugars. As some sugars require more mass to generate the full absorbance range, the actual amounts used for the standard curve may vary.
5. Set up sample assays by adding a volume containing ~5 µg of the derivatized polysaccharide to three sample tubes and bring the total volume to 100 µL with water. Alternatively, if the polysaccharide concentration in the sample is unknown, perform a series of 4-fold dilutions. Test 100 µL of each dilution in triplicate.
6. Prepare fresh resorcinol at 6 mg/mL in deionized (dI) water immediately before use. Vortex until the resorcinol is in solution. Add 100 µL of 6 mg/mL resorcinol to each tube.
7. Carefully pour the estimated amount of 75% sulfuric acid into a small beaker.
  NOTE: Wear a lab coat, nitrile gloves, and safety glasses. Be careful of drips, spills, and splashes. Keep wet paper towels handy to wipe up any drips. As the activity of the sulfuric acid changes on extended exposure to air, use a uniform mixture of sulfuric acid for the entire assay.
8. Using a repeat pipettor, uniformly add 300 µL of 75% sulfuric acid to each tube. Vortex the tubes vigorously to mix well, pointing the tube away while vortexing. Place the tubes in a heater block at a steady pace in sequential order. Once all the tubes are in, set the timer for 3 min immediately.
9. At 3 min, remove the tubes at a steady pace in the same order, and place them directly in a rack in an ice water bath. Leave the tubes until they are ice cold. Remove the tubes and allow them to equilibrate to room temperature for ~5 min to prevent condensation on the cuvette during reading.
10. Set a UV/VIS spectrophotometer to read the absorbance at 430 nm using a 10 mm pathlength cuvette. Blank with a zero standard tube. Read the absorbance of all the tubes at 430 nm.
  NOTE: Disposable plastic cuvettes are convenient to use.
11. Construct a standard curve by plotting µg of carbohydrate standard vs. A₄₃₀. See Figure 4 for a typical standard curve using glucose as the reference standard.
12. Use the sample assay tubes with A₄₃₀ values falling within the linear range of the standard curve, calculate the µg amount of the unknown polysaccharide in the sample assay tubes from the standard curve equation. Determine the concentration of the unknown polysaccharide from the volume of the unknown added, accounting for dilutions. Convert the concentration to mg/mL or µM repeat units as required.
Hydrazide assay using trinitrobenzene sulfonic acid (TNBS)
1. Prepare 0.9% NaCl containing 0.02% sodium azide (Sample buffer) by dissolving 9 g of NaCl and 200 mg of sodium azide in dI H₂O to a final volume of 1 L.
2. Prepare 0.1 M sodium borate, pH 9 (Assay buffer), by mixing 100 mL of 0.5 M sodium borate, pH 9, with 400 mL of dI H₂O. Confirm that the solution pH is 9 ± 0.1; adjust if necessary.
3. Prepare 1% TNBS by diluting 200 µL of 5% 2,4,6-trinitrobenzene sulfonic acid solution to 1 mL with dI H₂O. Mark the tube as 1% TNBS and store at 4 °C in the dark for a week.
4. Prepare 50 mM ADH stock (equivalent to 100 mM hydrazide).
  1. Weigh out 871 mg of adipic dihyrazide (ADH) powder using an analytical balance. Dissolve the powder in a reagent bottle by adding Sample buffer to 100 mL with the aid of a top loader balance.
  2. Label the bottle as 100 mM hydrazide/50 mM ADH. Cap the bottle tightly and store at 4 °C for 1 year.
5. Prepare hydrazide standards (0.1, 0.2, 0.3, 0.4, 0.5, and 0.6 mM hydrazide).
  1. Prepare the 6 hydrazide standards by diluting the 100 mM hydrazide stock with Sample buffer with the aid of a top loader balance. Prepare 100 mL of each standard to minimize concentration error. Tightly close the bottles and store at 4 °C for 1 year.
6. Setting up assay reactions
  NOTE: The TNBS assay is run at a reaction volume of 1 mL. Each assay tube consists of 100 µL of a sample (or a standard), 875 µL of Assay buffer, and 25 µL of 1% TNBS solution. All assay reactions (for both samples and standards) are set up in triplicate.
  1. Label 3 borosilicate glass tubes (12 x 75 mm) for each standard, including the zero standard. Sort and arrange the standard tubes in tube rack in order of increasing concentration. Use a calibrated 100 µL or 200 µL micropipette to accurately add 100 µL of the standards to each corresponding tube. For the zero standard, use 100 µL of Sample buffer.
  2. Label 3 borosilicate glass tubes (12 x 75 mm) for each diluted sample to be assayed. Sort and arrange the sample tubes in the tube rack accordingly. Use a calibrated 100 µL or 200 µL micropipette to accurately add 100 µL of the sample to each corresponding sample tube.
  3. Use a calibrated 1000 µL micropipette to accurately add 875 µL of Assay buffer to all assay tubes: the standards and the samples.
7. To start the assay reaction, use a calibrated 100 µL micropipette to accurately add 25 µL of 1% TNBS to each assay tube. Start from the zero standard tubes, move to the standard tubes in order of increasing concentration, then to the sample tubes according to the pre-determined order. Change tips when starting a new standard or a new sample and keep the time spent in adding TNBS to all the tubes to within 5 min.
  1. Vortex all assay tubes for 2 s at high speed or at a speed setting allowing the liquid inside the assay tube to swirl upward to reach a height of 1/2 inch from the tube opening.
  2. Record the assay start time and set the timer to 2 h. Place the assay tube rack in the dark at room temperature for 2 h. When the time is over, vortex all the tubes one more time and proceed to data collection.
8. Data collection
  1. Let the UV/VIS spectrophotometer warm up and the baseline stabilize. Set the detection wavelength at 500 nm for the hydrazide assay. Use a 1 mL quartz cuvette of 1 cm pathlength for all absorbance measurements for the entire assay.
  2. Start the data collection by transferring a zero standard assay to the cuvette; blank the instrument (set absorbance to zero).
  3. Perform a single read on each tube and record the absorbance values in a data table. Remove any residual liquid from the cuvette before reading a new sample. Start from the zero standards, move to the standards of increasing concentration, and then to the samples. Once started, perform all steps efficiently without stopping and read all tubes within 10 min.
9. Analyzing sample data
  1. Create a standard curve by plotting mM hydrazide standard vs. A₅₀₀. Find the standard curve equation in the form of y = ax + b, where y represents mM hydrazide and x represents A₅₀₀. See Figure 4 for a typical standard curve.
  2. Calculate mM hydrazide in the samples using the standard curve equation, adjusting for the dilution factors. Choose only the sample assay tubes with A₅₀₀ values falling within the linear range of the standard curve for the calculation.
  3. Calculate the molar ratio of hydrazide/polysaccharide using equation (1).
    Hydrazide/polysaccharide = h / c × MW (1)
    Where h is the mM hydrazide, c is the mg/mL concentration of the polysaccharide, and MW is the polysaccharide molecular weight in kDa.
  4. Calculate the hydrazide labeling density per 100 kDa of polysaccharide using equation (2).
    Labeling density per 100 kDa polysaccharide = h / c × 100 (2)
    Where h is the mM hydrazide, and c is the mg/mL concentration of the polysaccharide.
    NOTE: For convenience, the polysaccharides can be considered to have a molecular weight of 100,000 daltons. This allows one to consider a "labeling density" in comparing the level of derivatization of various polysaccharides.
  5. Calculate the hydrazide labeling density as weight percent ADH.
    1. Determine the effective mg/mL concentration of ADH by using equation (3).
      mg/mL ADH = (mM hydrazide / 1000) × 174 (3)
      where 174 is the MW of ADH.
    2. Calculate the weight % ADH by using equation (4).
      weight % ADH = (mg/mL ADH) / (mg/mL polysaccharide) × 100 (4)

Representative Results

To illustrate the activation and derivatization of a polysaccharide using CDAP chemistry, dextran was activated at 0.25 and 0.5 mg CDAP/mg dextran. For each reaction, a 10 mg/mL dextran solution in water was chilled on ice, and 1/10^th volume of a 2.5 M DMAP stock (prepared as described in section 3) was added. The final solution was brought to pH 9 by the addition of 0.1 M NaOH in 10 µL aliquots. The solution was chilled and stirred, CDAP added, and the pH maintained at pH 9 by adding 10 µL aliquots of 0.1 M NaOH for 15 min. Only 0.25 mL of 0.5 M ADH at pH 9 was added (less than the usual amount) and the reaction allowed to proceed overnight at 4 °C.

The labeled dextran was then sequentially dialyzed against 1 M NaCl, 0.15 M NaCl, and water as described in section 6. The ADH-dextran was then assayed for dextran using the resorcinol/sulfuric acid assay (section 7.2). A typical standard curve using glucose as the sugar standard is shown in Figure 4A. The hydrazide content was determined using the TNBS assay described in section 7.3. A typical hydrazide standard curve using ADH as the standard is given in Figure 4B.

Representative calculations from the activation of dextran at the two levels of activation are shown in Figure 4A,B. The data are presented as both hydrazides per 100 kDa of dextran polymer and as a weight percent of ADH to dextran, as described in sections 7.9.3.4 and 7.9.3.5, respectively, in Figure 4C. The degree of derivatization approximately doubled as the CDAP ratio was doubled.

Figure 1: Chemical structure of CDAP. CDAP = 1-cyano-4-dimethylaminopyridine tetrafluoroborate. Please click here to view a larger version of this figure.

Figure 2: Process of CDAP activation and conjugation. The process is conceptually divided into two phases, with the activated polysaccharide common to both. Under basic conditions, CDAP activates polysaccharide hydroxyls, releasing DMAP (reaction 1). CDAP hydrolysis also releases DMAP (reaction 3). Although a cyano-ester is shown, this may not be the actual intermediate. The intermediate is, therefore, referred to as (CDAP) "activated" polysaccharide. During the first activation phase, the activated polysaccharide can hydrolyze (reaction 4) or undergo side reactions (reaction 5). In the second conjugation phase (reaction 2), the activated polysaccharide reacts with an amine to form a stable isourea bond in addition to reactions 4 and 5. Abbreviations: CDAP = 1-cyano-4-dimethylaminopyridine tetrafluoroborate; DMAP = 4-dimethylaminopyridine; R-NH₂ = amine. Please click here to view a larger version of this figure.

Figure 3: CDAP activation and conjugation. The process requires balancing CDAP reactivity with the polysaccharide, the stability of the CDAP and activated polysaccharide, as well as the reactivity of the activated polysaccharide with that of the amine. Please click here to view a larger version of this figure.

Figure 4: Representative results for CDAP activation of dextran. Typical standard curves for the (A) resorcinol/sulfuric acid and (B) TNBS assays. The assay results for dextran activated with 0.25 and 0.5 mg CDAP/mg dextran are shown. Glucose was used as the standard for the resorcinol assay. Dextran, in mg/mL, is divided by 100 kDa to give a molar concentration. The hydrazide concentration is determined using ADH as the standard and the results expressed as µM Hz. (C) Calculation of hydrazide: dextran ratios.The level of derivatization was calculated as hydrazides per 100 kDa of dextran to facilitate the comparison between polymers of different average molecular weights. The % weight ratio of g ADH/g dextran was calculated using a MW of 174 g/mole for ADH. Please click here to view a larger version of this figure.

Discussion

CDAP is a convenient reagent to derivatize and conjugate polysaccharides. This article describes the general method to use CDAP to derivatize polysaccharides with hydrazides (PS-ADH) and incorporates recently published improvements⁸. First, the technique emphasizes the importance of maintaining the target pH to control the activation process. We found that while many common buffers interfere with the CDAP activation reaction, DMAP could successfully be used as the buffer to manage the pH⁸. Furthermore, DMAP is already a reaction byproduct of CDAP activation. Finally, buffering the polysaccharide solution with DMAP before adding the CDAP facilitates precise targeting and maintenance of the reaction pH. As we describe, it is useful to adjust the pH of the concentrated DMAP stock solution such that when diluted, it reaches the targeted pH. Secondly, performing the process in the cold slowed the reaction time, making the activation process less frenetic and more forgiving. Lower temperature decreased the rate of CDAP hydrolysis, and the optimal activation time at pH 9 increases from ~3 min to ~15 min. In addition, less CDAP is required to achieve the same level of activation than when performed at room temperature.

ADH-derivatized polysaccharides can be conjugated to proteins using carbodiimides (e.g., EDAC)⁷. For example, several licensed Haemophilus influenzae b (Hib) vaccines use the polyribosylribitolphosphate (PRP) derivatized with ADH to conjugate to tetanus toxoid using EDAC. CNBr was initially employed, but CDAP is a much easier reagent to use for this purpose. In our experience, a good target range for ADH derivatization is 10-30 hydrazides per 100 kDa polysaccharide or ~1-3% ADH by weight.

The same process can be used to derivatize polysaccharides with primary amines by substituting the ADH for a diamine. It is recommended to use hexane diamine to derivatize polysaccharides with amines⁸. The aminated polysaccharide (PS-NH₂) can be conjugated using reagents developed for protein conjugation¹¹. Typically, the PS-NH₂ is derivatized with a maleimide (e.g., succinimidyl 4-[N-maleimidomethyl]cyclohexane-1-carboxylate (SMCC) or N-γ-maleimidobutyryl-oxysuccinimide ester (GMBS)), and the protein is thiolated (e.g., with succinimidyl 3-(2-pyridyldithio)propionate (SPDP)). Thiol-maleimide chemistry is very efficient.

Proteins can also be directly coupled to CDAP-activated polysaccharides via the ɛ-amine on lysines. While the activation protocol used is generally similar to the one described here, it is necessary to optimize the level of activation, polysaccharide and protein concentration, as well as the protein:polysaccharide ratio⁵^,⁶^,⁸.

Dextran is one of the easiest polysaccharides to activate with CDAP due to its relatively high density of hydroxyl groups, but some polysaccharides, such as Vi antigen, can be challenging. Consequently, there is no single “best” protocol for CDAP conjugation directly to proteins. We suggest first developing a protocol to achieve suitable levels of activation, as determined by the extent of hydrazide derivatization, and then proceeding to direct protein conjugation to CDAP-activated polysaccharide.

Divulgazioni

The authors have nothing to disclose.

Acknowledgements

The work described here was funded by Fina Biosolutions LLC.

Materials

Acetonitrile	Sigma	34851
Adipic acid dihydrazide	Sigma	A0638	MW 174
Amicon Ultra 15 10 kDa	Millipore	UFC901008	MW cutoff can be 30 kDa for 200 kDa PS
Analytical balance
Autotitrator or electronic pipet
Beaker 2-4 L
CDAP	SAFC	RES1458C	Sigma
DMAP	Sigma	107700	MW 122.2
Flake ice
HCl 1 M	VWR	BDH7202-1
Micro stir bar	VWR	76001-878
Microfuge tube (for CDAP)	VWR	87003-294
NaCl	VWR	BDH9286
NaOH 1 M	Sigma	1099130001
NaOH 10 M	Sigma	SX0607N-6
pH meter
pH probe	Cole Parmer	55510-22	6 mm x 110 mm Epoxy single junction
pH temperature probe
Pipets & tips
Saline or PBS
Small beaker 5-20 mL	VWR	10754-696	A 10 mL beaker allows room for pH probe & pipet
Small ice bucket
Small spatula
Stir plate
Resorcinol assay
Combitip	Eppendorf	10 ml
DI water
Dialysis tubing	Repligen	132650T	Spectra/Por 6-8kDa
Dialysis tubing clips	Repligen	142150
Heating block
Nitrile gloves	VWR
Repeat pipettor	Eppendorf	M4
Resorcinol	Sigma	398047
Sugar standard		As appropriate
Sulfuric acid 75%	VWR	BT126355-1L
Timer
TNBS assay
Adipic dihydrazide	Sigma	A0638	MW 174
Borosilcate test tubes 12 x 75	VWR	47729-570
Sodium borate, 0.5 M pH 9	Boston Biologicals	BB-160
TNBS 5% w/v	Sigma	P2297	MW 293.17

Riferimenti

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Citazione di questo articolo

Lees, A., Zhou, J. Activation and Conjugation of Soluble Polysaccharides using 1-Cyano-4-Dimethylaminopyridine Tetrafluoroborate (CDAP). J. Vis. Exp. (172), e62597, doi:10.3791/62597 (2021).