Open Access This article is
- freely available
Membranes 2018, 8(3), 85; https://doi.org/10.3390/membranes8030085
Dual Functional Ultrafiltration Membranes with Enzymatic Digestion and Thermo-Responsivity for Protein Self-Cleaning
Institute for Sustainable Industries and Liveable Cities, College of Engineering and Science, Victoria University, P.O. Box 14428, Melbourne, VIC 8001, Australia
Institute for Frontier Materials, Deakin University, Waurn Ponds, Geelong, VIC 3216, Australia
Authors to whom correspondence should be addressed.
Received: 24 August 2018 / Accepted: 17 September 2018 / Published: 19 September 2018
Controlling surface–protein interaction during wastewater treatment is the key motivation for developing functionally modified membranes. A new biocatalytic thermo-responsive poly vinylidene fluoride (PVDF)/nylon-6,6/poly(N-isopropylacrylamide)(PNIPAAm) ultrafiltration membrane was fabricated to achieve dual functionality of protein-digestion and thermo-responsive self-cleaning. The PVDF/nylon-6,6/PNIPAAm composite membranes were constructed by integrating a hydrophobic PVDF cast layer and hydrophilic nylon-6,6/PNIPAAm nanofiber layer on to which trypsin was covalently immobilized. The enzyme immobilization density on the membrane surface decreased with increasing PNIPAAm concentration, due to the decreased number of amine functional sites. An ultrafiltration study was performed using the synthetic model solution containing BSA/NaCl/CaCl2, where the PNIPAAm containing biocatalytic membranes demonstrated a combined effect of enzymatic and thermo-switchable self-cleaning. The membrane without PNIPAAm revealed superior fouling resistance and self-cleaning with an RPD of 22%, compared to membranes with 2 and 4 wt % PNIPAAm with 26% and 33% RPD, respectively, after an intermediate temperature cleaning at 50 °C, indicating that higher enzyme density offers more efficient self-cleaning than the combined effect of enzyme and PNIPAAm at low concentration. The conformational volume phase transition of PNIPAAm did not affect the stability of immobilized trypsin on membrane surfaces. Such novel surface engineering design offer a promising route to mitigate surface–protein contamination in wastewater applications.
Keywords:thermo-responsive; ultrafiltration; enzymes; self-cleaning; nanofibers
Non-specific surface–protein interactions at the membrane interface during ultrafiltration (UF) leads to permanent fouling, by accumulation of protein contaminants on the surface or pores of the membrane . Membrane fouling by proteins block the membrane pores and eventually form cake layer that rapidly decline membrane permeability, increase the cleaning frequency and reduce membrane performance [2,3]. One of the most adaptable methods to decrease fouling and self-clean the membranes is to modify the membrane surface functionalities by incorporating self-cleaning materials such as hydrophilic copolymers [4,5], amphiphilic copolymers , zwitterionic compounds , metal oxides , biocatalytic enzymes [1,9], and responsive materials [5,10,11]. Self-cleaning materials are a class of materials with intrinsic ability to remove any contaminant from their surfaces via various mechanisms .
Enzymes are biocatalizers that act as biochemical catalysts of specific substrates to produce individual products. Proteolytic enzymes have attracted attention as self-cleaning compounds that can breakdown and remove the protein foulants from the membrane surface [1,13]. To overcome self-hydrolysis of free enzymes in solution leading to instability, deprived performance and poor reusability , enzymes may be immobilized onto suitable substrates. The nature and properties of the substrates play an important role in enhancing the loading of enzymes, enzyme stability and its activity over time and cleaning cycles .
Electrospun nanofibers, owing to their high surface-to-volume ratio, are considered to be one of the most appropriate substrates for enzyme immobilization providing high loading of enzymes and improved stability , as well as great structural versatility and facile control on surface chemistry [17,18]. The nanofiber membranes possess high porosity and pore interconnectivity that provide low hindrance to mass transfer making it suitable for filtration [19,20]. The activity of enzyme immobilized onto nanofibers was found to be greater than that of the activity of enzymes immobilized onto commercially cast membranes, owing to the high surface area providing more active sites for enzyme immobilization [9,21,22]. Furthermore, the enzyme immobilized onto nanofibers demonstrated good operational reusability. For example, trypsin immobilized onto polyethylene terephthalate (PET)/poly (lactic acid) (PLA) nanofiber mats and chitosan nanofibers presented 80% (eleven cycles) and 97% (five cycles) reusability, respectively [23,24]. Nanofibers are typically used as the top functional layer together with a support layer underneath, during the treatment of complex wastewater . Despite showing enhanced membrane antifouling performance and enzyme reusability, the reported biocatalytic UF membranes exhibited low permeability [1,26,27]. Thus, biocatalytic fouling resistant membranes with stable enzyme immobilization onto the surface and altered pore structure offering high permeability and long-term operational stability are desired. Since enzymes are susceptible to loss in activity over time [9,28], an additional self-cleaning material that provide facile membrane cleaning may be incorporated to achieve enhanced performance.
Thermo-responsive polymers are considered among the promising antifouling materials that offer facile temperature-based cleaning for membranes . With a lower critical solution temperature (LCST) of about 32 °C in an aqueous solution, poly(N-isopropylacrylamide) (PNIPAAm) is a well-recognised temperature-sensitive polymer [30,31]. Below LCST, the PNIPAAm polymer chains are more hydrophilic having an extended conformation in water and above LCST, they become less hydrophilic forming a dehydrated compact structure exhibiting a sharp reversible volume-phase conformational transition providing strong inherent washing force. On one hand, the self-cleaning behaviour of the PNIPAAm containing membrane could be attributed to the enhanced hydrophilicity below its LCST, thus facilitating foulants desorption from the surface. For example, PNIPAAm grafted polydopamine/PET UF membranes recovered 90% of the initial flux at 20 °C compared to unmodified PET membrane that showed only 76% flux recovery, ascribed to the enhanced surface hydrophilicity . Similarly, a flux recovery of 92% was achieved for the poly (vinylidene fluoride) (PVDF)/TiO2-g-PNIPAAm nanocomposite membranes compared to 47% flux recovery for the control PVDF membranes at 23 °C . On the other hand, the thermo-switchable characteristic of PNIPAAm providing strong inherent washing force was exploited to remove the membrane foulants in UF, exhibiting self-cleaning property. For example, the polyethylene membrane onto which PNIPAAm was grafted, showed 97% flux recovery via applying a temperature-change (25 °C/35 °C) cleaning method to the bovine serum albumin (BSA) fouled membranes . Similarly, the PNIPAAm-grafted ZrO2 membrane showed 80% flux recovery after temperature-change cleaning (25 °C/35 °C) of BSA fouled membranes . However, the combined self-cleaning effect of PNIPAAm and biocatalytic enzymes has not been explored so far and the impact of one material on the other with respect to filtration and self-cleaning effect was not investigated. In this study, a new biocatalytic PVDF/nylon-6,6/PNIPAAm composite UF membrane was fabricated by covalently immobilizing trypsin (TR) enzyme onto functional nanofibrous surface of PVDF/nylon-6,6/PNIPAAm membrane, to achieve dual functionality of protein-digestion and thermo-responsivity for self-cleaning effect. The structural and functional properties of the as-prepared composite membranes were investigated and correlated to the membrane performance in UF fouling experiments with intermediate temperature cleaning. Also, the impact of thermo-switchable volume-phase transition on the stability of immobilized enzymes was studied. Figure 1 shows the schematic of membrane self-cleaning using enzymes and thermo-responsive PNIPAAm polymer via protein-digestion and volume phase transition mechanisms, respectively.
2. Experimental Section
PVDF Kynar 761 with a melting point 165–172 °C was purchased from Arkema Pte. Ltd. (Singapore). Trypsin (from porcine pancreas) was purchased from Wako pure chemical industries Ltd. (Osaka, Japan). PNIPAAm, (Mw 113 g/mol), polyamide-6,6 (nylon-6,6) (Mw 262.35 g/mol), poly(vinylpyrrolidone) (PVP-K-40) (Mw 40,000), 1-ethyl-3-(3-dimethylaminopropyl) carbodiimide (EDC), BSA (Mw 66 kDa) as model protein, N-hydroxysuccinimide (NHS), formic acid (>95%), N,N′-dimethylacetamide (DMAC) (99.8%), trichloroacetic acid (TCA) (99%), ethanol (75%), sodium chloride (NaCl), glycerol (>99.5%) and calcium chloride (CaCl2) were purchased from Sigma Aldrich (St. Louis, MO, USA) and was used as received. Deionized (DI) water was obtained from the Milli-Q plus system (Millipore, Bedford, MA, USA) and used in all experiments.
2.2. Preparation of PVDF/nylon-6,6/PNIPAAm Membrane
The thermo-responsive PVDF/nylon-6,6/PNIPAAm composite membrane was prepared using a similar method used in our earlier study . Concisely, the preparation of composite membrane was carried out using three consecutive steps, (a) construction of thermo-responsive functional nanofiber mat by electrospinning a mixed solution of two different PNIPAAm concentrations (2 and 4 wt % PNIPAAm) and 10 wt % nylon-6,6 in formic acid, at 0.25 mL/h flow rate and 17 kV voltage with 150 mm tip to collector distance, (b) conventional casting of the PVDF dope solution prepared by continuous stirring of 8 wt % PVP and 18 wt % PVDF in DMAC solvent at 50 °C overnight, on to the nanofiber mat and (c) immersion of the cast and nanofiber layers together into a coagulation tank of DI water to remove the residual solvent via phase inversion. Further, the post-treatment of nascent membranes was performed by immersing them in to a mixture of ethanol, glycerol and DI water in the ratio 1:2:2 (vol %) and was dried finally before characterisation. Also, the control PVDF/nylon-6,6 membrane was fabricated without the addition of PNIPAAm.
2.3. Preparation of Biocatalytic PVDF/nylon-6,6/PNIPAAm Membranes
The TR enzyme immobilization on to the as-prepared membranes with no PNIPAAm (PN0), 2 wt % (PN2) and 4 wt % (PN4) PNIPAAm were attained by EDC/NHS immobilization reaction using a similar method used in our previous study , to form PN0-TR, PN2-TR and PN4-TR membranes, respectively. Firstly, 1 mg/mL TR solution was reacted with EDC/NHS (4:1) aqueous solution for about 1 h at room temperature, to activate the enzyme carboxyl groups. Secondly, the activated enzymes were covalently attached onto the PN0-TR, PN2-TR and PN4-TR membranes by reacting with the primary amines on the membrane surface for 12 h at 4 °C. Finally, the absorbed TR was removed by rinsing the membranes with DI water. The decrease in enzyme concentration in solution before and after contact with the membrane was used to calculate the enzyme immobilization efficiency.
2.4. Membrane Characterization
Scanning electron microscopy (SEM) (SUPRA 55VP, ZEISS, Jena, Germany) was used to study the surface morphology of the as-prepared biocatalytic membranes. The accelerating voltage was set to 5 kV with 10 mm working distance for the observation. The membrane samples were prepared prior to observation by sputter coating them using Leica EM ACE600 (Leica microsystems, Sydney, NSW, Australia), in high vacuum with a gold layer of 5 nm thickness. The observed SEM images were used to evaluate the average nanofiber diameters of the membranes using ImageJ software. Porometer 3Gzh (Quantachrome, Boynton beach, FL, USA) was used to measure the membrane pore size and its distribution. The membranes (25 mm diameter each) were first wetted with Porofil™ liquid and positioned in the sample holder after which it was exposed to 6.4 to 34 bar pressures for wet and dry run. The measurement was carried out three times for each membrane to obtain the average pore size. CAM101 optical contact angle meter (KSV Instruments, Helsinki, Finland) was used to measure the dynamic water contact angles (CAw) of the as-prepared membranes and to investigate the switchable surface hydrophilicity at 22 °C (below LCST) and 50 °C (above LCST). The required temperature of the membrane samples was achieved by adjusting the voltage of the source meter connected to the heating pad on which the samples are mounted. Prior optimisation of corresponding temperatures and feed voltages of the heating mats were established before mounting the heating pad on the contact angle meter. The measurement was performed by pasting rectangular strips of each membrane sample on to the sample stage and dispensing 4 µL water droplet onto the membrane surface through a needle. Each measurement was recorded every 5 s over the duration of 60 s.
2.5. Quantification of Immobilized TR and Its Activity against BSA
UV–Visible spectrophotometer (Model UV-1800, Shimadzu, Columbia, SC, USA) was used to measure the decrease in TR concentration of the test solution before and after filtration experiments at the wavelength of 280 nm, owing to its simplicity, reliability and convenience. The immobilized TR surface density of the thermo-responsive composite membranes was calculated similarly to the method reported in literature . Furthermore, the enzymatic activities of biocatalytic thermo-responsive membranes and free TR were calculated by measuring their hydrolytic activities via previously described method using 1 wt % BSA solution as the substrate . Briefly, the immobilized and free TR were first reacted with the BSA solution for up to 1 h at 37 °C after which the reaction was terminated using 5 wt % TCA and then centrifuged at 2000× g to measure the absorbance of the supernatant containing hydrolytic products using UV–Visible spectrophotometer (280 nm). The supernatant of the centrifuged solution after similar reaction without TR was used as the blank. In this study, 0.1 increase in absorbance of the hydrolytic products represents one digestion unit (DU) that denotes an increase in the amount of substrate digested by the enzymes via hydrolysis. However, the measured hydrolytic activity of the immobilized enzymes was normalized to 100% as a benchmark, based on the literature that showed superior activity and operational stability of the enzymes immobilized on to nanofibrous substrate .
2.6. Fouling Studies
A cross flow UF system (42 × 10−4 m2 effective area; 12.6 cm/s flow velocity) was used to evaluate the antifouling and self-cleaning properties of the biocatalytic thermo-responsive membranes. To simulate a practical fouling environment in wastewater treatment, a complex synthetic feed solution containing 1 mg/mL BSA (model protein), 1 mM CaCl2 and 7 mM NaCl in DI water with pH 7.8 (optimum TR pH range 7.5–8.5) was used in this study . The addition of NaCl and CaCl2 to the protein feed solution greatly increased the potential for surface fouling and simulated a practical fouling environment. It was demonstrated that a thicker and more compact fouling layer was formed on the membrane surface through the calcium-induced protein aggregation via (a) forming protein−Ca2+−protein complexes and (2) intramolecular electrostatic shielding of the protein negative charges by Ca2+ . Although the current study focused on protein rich synthetic solution, future work studying the novel membrane’s ability to perform in such complex real water matrices for specific applications could be performed. Initially, each membrane was compacted at 120 kPa for 10 min at RT using DI water and then exposed to DI water containing 7 mM NaCl at 100 kPa for 15 min to measure the clean water permeance (Pw) in L m−2 h−1 calculated by the following equation:where V stands for the permeate volume in L, A stands for the membrane area in m2, t stands for the permeation time in h and p stands for the constant pressure (1 bar). Each cycle of the 2 cycle UF experiment includes the filtration of the as-prepared feed solution at 22 °C for 1 h followed by an intermediate temperature cleaning with DI water at 22 °C for 15 min. The cycle number was denoted by ‘n’. The fouling studies were carried out by performing the UF experiment three times for each of the membranes and was averaged to ensure reproducibility. The rate of permeance decline (RPD) after each cycle was determined as a measure of protein fouling using the equation,where Pe(n) stands for the final feed permeance in nth cycle. Further, the membrane self-cleaning property was studied by calculating the permeance recovery after the intermediate temperature cleaning at 22 °C, using the equation,where Pw(n) stands for the clean water permeance in nth cycle. Also, the fouling parameters namely irreversible fouling (IF), reversible fouling (RF) and total fouling (TF) for each cycle was computed by the following equations:where Ps stands for the initial feed permeance in each cycle and Pe stands for the final feed permeance in each cycle. Finally, the membrane surfaces were visualised after 2 cycles of filtration using SEM and the antifouling and self-cleaning properties of the enzyme immobilized membranes with and without PNIPAAm was compared. Further, to investigate the combined antifouling and self-cleaning effects of protein-digestive enzymes and thermo-responsive PNIPAAm, 2 filtration cycles each including 1 h filtration of the as-prepared feed solution at 22 °C followed by an intermediate temperature cleaning with DI water at 50 °C for 15 min were also performed and their respective RPD was calculated for comparison.
2.7. Storage Studies and Effect of Thermo-Responsivity on Enzyme Stability
The storage study for the biocatalytic membranes were conducted by storing them under refrigeration at 4 °C and RT (22 °C) up to two weeks during which the enzyme activity was measured at regular intervals. Further, the effect of thermo-switchable volume phase transition of the PNIPAAm on enzyme stability was examined by measuring the hydrolytic activities of the as-prepared membranes (a) before and after treating the membranes for 5 min at 50 °C and (b) over six consecutive reuse cycles before treating the membranes for 5 min at 50 °C and after the treatment. These studies were conducted to investigate if the volume phase transition during thermo-switchable cleaning affects the stability of enzymes immobilized on to the membrane surfaces; 5 min treatment at 50 °C is exposing the membrane samples to DI water maintained at 50 °C and mild stirring at 100 rpm for 5 min.
3. Results and Discussion
3.1. Enzyme Distribution on Membrane Surface
The distribution of enzymes on the surface of PVDF/nylon-6,6/PNIPAAm and PVDF/nylon-6,6 membranes were analysed using the SEM imaging and shown in Figure 2. All the TR immobilized membranes with no PNIPAAm, 2 and 4 wt % PNIPAAm showed homogenous nanofiber structure with an average nanofiber diameter of 87 ± 17 nm, 180 ± 15 nm and 314 ± 20 nm, respectively. The membrane with 4 wt % PNIPAAm show nano-branched structure with beads and clusters in some nanofibers that could be attributed to the uneven distribution of enzymes; while the membranes with no PNIPAAm and 2 wt % PNIPAAm showed homogenous enzyme attachment as seen in Figure 2. These clusters were formed due to possible aggregation of TR by randomized attachment points on the membrane implying the lack of control on enzyme immobilization . Further, the thickness of the biocatalytic membranes with no PNIPAAm, 2 and 4 wt % PNIPAAm was measured from the cross sectional SEM micrographs to be 249 ± 9 µm, 257 ± 6 µm and 265 ± 11 µm, respectively.
3.2. Surface Density of Immobilized Enzyme
The density of immobilized TR on the surface of membranes was measured to study the amount of covalently attached enzymes and the results are presented in Figure 3. It was observed that the surface density of immobilized TR decreased as the PNIPAAm concentration in the membrane increased. This can be attributed to the incorporation of PNIPAAm in to the membrane which decreased the availability of surface amine functional groups from nylon-6,6 used for enzyme attachment via carbodiimide chemistry using EDC and NHS. The surface densities of immobilized TR on PVDF/nylon-6,6/PNIPAAm membranes with no PNIPAAm, 2 and 4 wt % PNIPAAm were 4.01 mg/m2, 3.43 mg/m2 and 2.87 mg/m2, respectively, which were higher than the reported values of 0.7 mg/m2 of TR immobilized PES membrane in the literature due to the nanofiber structure providing a higher surface area for enhanced immobilization . Among the prepared membranes, the control membrane without PNIPAAm had higher surface density of enzymes.
3.3. Membrane Characterization
To evaluate the hydrophilicity and responsivity of biocatalytic thermo-responsive membranes, the dynamic water contact angles (CAw) were measured over 60 s at 22 °C and 50 °C and are given in Figure 4a,b, respectively. The CAw for the PNIPAAm containing membranes at 22 °C exhibit a slightly faster attenuation compared to control membrane, as shown in Figure 4a. This decreasing tendency could be due to the addition of PNIPAAm that has a hydrophilic extended conformation below its LCST (32 °C) which absorbs water by forming hydrogen bonds between the amide groups of PNIPAAm and water, in spite of having lesser immobilized enzymes compared to control membrane. Also, at 22 °C, the biocatalytic PVDF/nylon-6,6/PNIPAAm membrane with 2 wt % PNIPAAm showed the lowest CAw of 13.6° compared to the membrane with 4 wt % PNIPAAm (18.4°) after 60 s, which may be ascribed to the increased amount of immobilized TR on the membrane surface. Figure 4b shows the dynamic CAw of the as-prepared membranes at 50 °C. For the PVDF/nylon-6,6 without PNIPAAm, the CAw attenuation was similar at both 22 °C and 50 °C. However, the initial CAw values for PNIPAAm containing membranes were higher at 50 °C compared to those at 22 °C, owing to the hydrophobic nature of the membrane above LCST that breaks the hydrogen bonds between amide groups of PNIPAAm and water molecules.
To investigate the volume-phase transition of the PNIPAAm around its LCST, the thermo-switchable CAw of the membranes was measured and compared in terms of initial CAw at 22 °C and 50 °C, as shown in Figure 4a,b, respectively. The biocatalytic membrane without PNIPAAm exhibited no CAw switchability; while the membranes with 2 and 4 wt % PNIPAAm exhibited switchable CAw from 43.5° to 59° and from 44.8° to 61.8°, respectively, between 22 °C and 50 °C. The slightly higher switchability of biocatalytic membrane with 4 wt % PNIPAAm compared to membrane with 2 wt % PNIPAAm is attributed to increased PNIPAAm concentration in the membrane. However, this CAw variation is more significant than the PVDF-g-PNIPAAm membrane reported in literature that exhibited switching CAw from 87.5° (22 °C ) to 89° (50 °C) .
The mean pore size and the distribution of the as-prepared composite membranes were measured by a capillary-flow porometer . The differential pore distributions of the membranes are presented and compared in terms of pore diameters in Figure 4c. The TR immobilized PVDF/nylon-6,6 membrane exhibited narrow distribution curve due to the homogenously attached enzymes; while the TR immobilized membranes with 2 and 4 wt % PNIPAAm exhibited bimodal distribution curves owing to the formation of non-homogenous pore structures due to TR immobilization. The TR immobilized membrane with 4 wt % PNIPAAm membrane showed slightly wider distribution, possibly due to the clustering of TR enzymes as observed in Figure 2. The mean pore size of the TR immobilized on PVDF/nylon-6,6/PNIPAAm membranes with no PNIPAAm, 2 and 4 wt % PNIPAAm were 44, 33 and 23 nm, respectively. The smaller pore size of the as-prepared membrane with 4 wt % PNIPAAm compared to those membranes with no PNIPAAm and 2 wt % PNIPAAm is ascribed to the formation of enzyme clusters on the membrane surface (Figure 2c).
3.4. Enzyme Activity Evaluation Across the Nano-Composite Membranes
Figure 4d show the results respective to the reaction time. The number of products formed by immobilized TR were noticed to be much greater than that of the free enzymes for all reaction times up to 60 min. For instance, at 60 min, the TR immobilized on to the membranes with no PNIPAAm, 2 and 4 wt % PNIPAAm produced about 7.5, 5.5 and 4.7 times more peptide products, respectively, than the free TR. It was also observed that the activity of immobilized TR increased with reaction time; while the activity of free enzymes increased initially but became stable in 10 min. This is due to the increased stability of immobilized TR that has greatly enhanced the enzymatic activity, whereas the free TR undergoes autolytic behaviour commonly known as self-digestion [39,40,41]. The results further revealed that the PVDF/nylon-6,6 membrane without PNIPAAm show superior enzyme activity than the PNIPAAm containing membranes, possibly due to high immobilization density (Figure 3).
3.5. Protein Fouling Studies
The combined enzymatic and thermo-responsive effect on surface–protein interaction of the as-prepared biocatalytic membranes was investigated by conducting the filtration experiments with and without temperature-change cleaning, i.e., two-cycle filtration with respective intermediate DI water cleaning at 22 °C and 50 °C.
Figure 5 shows the results of two consecutive filtration cycles with intermediate DI water cleaning at 22 °C presented in terms of water permeance and RPD as a measure of protein fouling, and PRR, IF, RF and TF, as measures of the self-cleaning ability of the membranes. The error bars in Figure 5 indicate the reproducibility of the results. As presented in Figure 5a, the biocatalytic membranes with 2 wt % (506 L m−2 h−1 bar−1) and 4 wt % (442 L m−2 h−1 bar−1) PNIPAAm exhibited slightly lower initial water permeance i.e., 13% and 24% lesser, compared to the membrane without PNIPAAm (581 L m−2 h−1 bar−1), which is attributed to the decrease in pore size due to the incorporation of PNIPAAm (Figure 4). Based on the permeance patterns observed for all membranes in Figure 5a, the RPD was calculated based on Equation (2) and presented in Figure 5b to indicate the resistance to protein fouling. During the first filtration cycle, the biocatalytic PVDF/nylon-6,6/PNIPAAm membranes with no PNIPAAm, 2 and 4 wt % PNIPAAm suffered fouling as indicated by an RPD of about 19%, 33% and 39%, respectively. The lower RPD of biocatalytic membrane without PNIPAAm suggests that the membrane with higher density of immobilized enzymes with increased proteolytic ability i.e., protein digestive feature, were able resist BSA fouling to a larger extent . Also, this result was found to be promising compared to the TR immobilized PMAA-g-PES UF membrane as reported in literature that showed 19.1% flux decline rate using 1 g/L BSA solution .
Further, during the second filtration cycle, the RPD values were 22%, 39% and 45% for respective biocatalytic membranes with no PNIPAAm, 2 and 4 wt % PNIPAAm, after temperature cleaning at 22 °C. Similar to first filtration cycle, the increasing RPD follows the decreasing trend of immobilized TR density on the membrane surface. The SEM micrographs of the fouled membranes are presented in Figure 6. Consistent to the permeance results, the biocatalytic PVDF/nylon-6,6/PNIPAAm membrane with 4 wt % PNIPAAm showed heavy fouling (Figure 6c) compared to that without PNIPAAm that exhibited much reduced protein deposition presenting clear surface after two filtration cycles (Figure 6a), followed by the membrane with 2 wt % PNIPAAm that showed regional accumulation of protein (Figure 6b).
The self-cleaning efficiency of the as-prepared biocatalytic membranes without temperature cleaning was quantified by computing PRR and fouling parameters namely IF, RF and TF. Figure 5c reveals that after the first filtration cycle, the biocatalytic membranes with no PNIPAAm, 2 and 4 wt % PNIPAAm were able to recover about 90%, 89% and 82% of the initial permeance, respectively. The greater permeance recovery of membranes with no PNIPAAm and 2 wt % PNIPAAm compared to that with 4 wt % PNIPAAm was attributed to the higher density of immobilized enzymes on the membrane surface that leads to breakdown of proteins into smaller polypeptides releasing them subsequently from the membrane surface. This result was found to be comparable with the TR immobilized PVDF MF membrane constructed using a complex method involving electron beam that showed 90% flux recovery after first filtration cycle with pure BSA solution of 3 g/L after backwashing with 120 mL of pure water every 1.6 L of filtration and self-cleaning through trypsin activation by immersing the fouled membrane into a buffered solution at 37 °C and pH 8.0 overnight . Similar trend was observed after the second filtration cycle with biocatalytic membranes with no PNIPAAm, 2 and 4 wt % PNIPAAm showing 85%, 78% and 76% permeance recovery, respectively. The corresponding IF and RF parameters are presented in Figure 5d. After the first filtration cycle, the membranes with no PNIPAAm and 2 wt % PNIPAAm reduced the IF by 43% and 41%, respectively, compared to that with 4 wt % PNIPAAm, explaining the higher PRR presented in Figure 5c. This result demonstrates that less permanent fouling occurs with more enzymes featuring the self-cleaning capacity of the biocatalytic membranes. Thus, the membranes with higher density of immobilized enzymes exhibited much lower TF, which is corresponding to their higher PRR. Here, depending on the self-cleaning ability and fouling mitigation, the biocatalytic PVDF/nylon-6,6 membrane without PNIPAAm was recognised as the best performing membrane.
To investigate the effect of PNIPAAm in the membrane matrix, the as-prepared biocatalytic PNIPAAm membranes were evaluated with the same filtration experiments, but involved temperature-change cleaning with DI water at 50 °C. The performance results in terms of permeance and RPD for two filtration cycles are given in Figure 7a,b, respectively. As shown in Figure 7a, the biocatalytic membranes with no PNIPAAm (556 L m−2 h−1 bar−1), 2 wt % (491 L m−2 h−1 bar−1) and 4 wt % (422 L m−2 h−1 bar−1) exhibited similar initial water permeance to those presented in Figure 5a, showing good repeatability. Also, these values were found to be higher than the initial water permeance (74.3 L m−2 h−1 bar−1) of PNIPAAm-g-ZrO2 membrane reported in literature . During the first filtration cycle, the RPD values for biocatalytic PVDF/nylon-6,6/PNIPAAm membranes with no PNIPAAm, 2 and 4 wt % PNIPAAm were 18%, 22% and 30%, which are found to be greater than the 10.9% reduction of flux of PNIPAAm-g-ZrO2 membrane reported in literature . Further, during the second filtration cycle, the RPD values were 22%, 26% and 33% for the respective membranes. The increasing trends of the RPD in both cycles are consistent with those in Figure 3 corresponding to increasing density of enzymes on the membrane surface. Nevertheless, these values were found to be lower than the RPD values reported with intermediate cleaning at 22 °C in Figure 5b. Also, from Figure 7a, during the second filtration cycle, the membranes with no PNIPAAm, 2 wt % and 4 wt % PNIPAAm recovered about 91%, 93% and 96% of the initial BSA permeance of first filtration cycle. Thus, in addition to the enzymatic protein digestive feature of the membrane, the temperature-change cleaning has confirmed the role of PNIPAAm on the antifouling and self-cleaning effects via thermo-switchable cleaning when the environment temperature switches from 22 °C to 50 °C. Overall, the as-prepared biocatalytic membrane without PNIPAAm revealed superior fouling resistance with reduced protein interactions compared to PNIPAAm containing membranes, indicating that higher degree of enzyme immobilization offers better self-cleaning than the combined effect at low enzyme and PNIPAAm concentrations. However, enzymes may suffer from deteriorating performance due to loss in biocatalytic activity over time [9,28] and hence further optimization of PNIPAAm concentration could be performed to achieve maximum thermo-switchable feature that further enhances the self-cleaning efficiency of membranes.
3.6. Storage Studies & Effect of Thermo-Responsivity on Enzyme Stability
The effect of storage time on the hydrolytic activities of the immobilized TR at 4 °C and RT (22 °C) were presented in Figure 8a,b, respectively. It was revealed that at both RT and 4 °C, the biocatalytic membrane without PNIPAAm retained about 81% and 78% of their initial enzymatic activities after 7 days, respectively, and about 71% and 69% of their initial activities after 14 days of storage. The activity results were found to be similar to the TR immobilized PVDF/nylon-6,6/chitosan membrane that was prepared in our earlier study  with 81% (RT) and 70% (4 °C) detainment of initial enzyme activity after 7 and 14 days of storage, respectively, showing good reproducibility. Thus, the prepared membranes may not require inconvenient refrigerated storage conditions and can be stored at RT. Similarly, the membranes with 2 and 4 wt % PNIPAAm stored at RT retained about 79% and 76% of the activity after 7 days, respectively, and about 69% and 64% of the initial activity after 14 days, respectively.
The effect of thermo-switchable volume phase transition of the as-prepared membranes on the activities of freshly immobilized and used TR enzymes was investigated and the respective results are given in Figure 8c,d. In Figure 8c, the enzyme activities of biocatalytic membranes with no PNIPAAm, 2 and 4 wt % PNIPAAm declined only about 9%, 11% and 12% after treating at 50 °C, which is similar to the storage data (Figure 8a,b) that did not affect the immobilized enzymes of PNIPAAm membranes. The enzyme activity of membrane with 4 wt % PNIPAAm declined most significantly by 12%, which is more than that without PNIPAAm (9%), possibly owing to the leaching of weakly attached TR enzyme clusters formed through aggregation on the membrane surface as observed in Figure 2. Similarly, in Figure 8d, the enzyme activities of as-prepared membranes after six consecutive reuse cycles and treatment at 50 °C dropped less than about 3% after treating at 50 °C. This could be due to the stable enzyme activity at both 22 °C and 50 °C temperatures and during conformational volume phase transition when the temperature switches from 22 °C to 50 °C. Further, from Figure 8d, the hydrolytic activities of immobilized enzymes declined with increasing reuse cycles (up to six cycles), that may be due to (a) the release of any enzymes that are weakly bound and (b) the gradual morphological change of fibers including swelling and disintegration due to high hydrophilicity . Also, the biocatalytic membranes with 2 and 4 wt % PNIPAAm show faster decline compared to the PNIPAAm-free membrane which may also be due to the loss of enzyme activity via change in nanofiber morphology via swelling and disintegration. Thus, the thermo-switchable volume phase transition of the as-prepared membranes was not found to affect the enzyme activity that was stable when temperature switched from 22 °C to 50 °C.
Biocatalytic membranes with and without PNIPAAm were successfully prepared by immobilizing trypsin enzymes onto a hydrophilic nylon-6,6/PNIPAAm nanofiber layer supported by a hydrophobic PVDF cast layer. It was demonstrated that superior enzyme loading on to the membrane without PNIPAAm can be achieved compared to PNIPAAm-containing membranes, owing to the amine-rich nanofibrous surface with high surface-to-volume ratio. The trypsin-immobilized membranes minimized surface–protein contamination on the surface via enzyme proteolytic digestion. As a result of the UF study conducted using model feed solution containing BSA, CaCl2 and NaCl, the biocatalytic membrane without PNIPAAm offered superior performance in separation and purification applications with more permeability and less fouling than the other membranes with PNIPAAm, demonstrating that higher degree of enzyme immobilization offers better self-cleaning than the combined self-cleaning of low concentrations of enzyme and PNIPAAm. Also, the thermo-switchable conformational volume phase transition of the as-prepared membranes did not affect the stability of surface immobilized enzymes. Hence, the fabrication of biocatalytic nanofibrous surface has greater potential to mitigate fouling and self-clean the fouled surfaces beyond membrane separation.
The experimental work was designed and carried out by A.V. under the guidance of L.F.D., M.C.D. and X.Y. The manuscript was written by A.V. and reviewed by all authors. All authors have given approval to the final version of the manuscript.
This research received no external funding.
This work was supported by Victoria India Institute via Victoria India Doctoral Scholarship. L. DUMEE acknowledges the Australian Research Council (ARC) for his DECRA fellowship (DE180100130). Xing Yang would like to acknowledge Victoria University for the Industry Postdoctoral Fellowship. The Microscopy platform at Deakin University and support from the technical team is also acknowledged.
Conflicts of Interest
The authors declare no conflict of interest.
|BSA||bovine serum albumin|
|LCST||lower critical solution temperature|
|SEM||scanning electron microscopy|
|CAw||water contact angle|
|RPD||rate of permeance decline|
|PRR||permeance recovery rate|
- Shi, Q.; Su, Y.; Ning, X.; Chen, W.; Peng, J.; Jiang, Z. Trypsin-enabled construction of anti-fouling and self-cleaning polyethersulfone membrane. Bioresour. Technol. 2011, 102, 647–651. [Google Scholar] [CrossRef] [PubMed]
- Jim, K.J.; Fane, A.G.; Fell, C.J.D.; Joy, D.C. fouling mechanisms of membranes during protein ultrafiltration. J. Membr. Sci. 1992, 68, 79–91. [Google Scholar] [CrossRef]
- Ho, C.-C.; Zydney, A.L. A combined pore blockage and cake filtration model for protein fouling during microfiltration. J. Colloid Interface Sci. 2000, 232, 389–399. [Google Scholar] [CrossRef] [PubMed]
- Zhao, Z.; Zheng, J.; Wang, M.; Zhang, H.; Han, C.C. High performance ultrafiltration membrane based on modified chitosan coating and electrospun nanofibrous pvdf scaffolds. J. Membr. Sci. 2012, 394, 209–217. [Google Scholar] [CrossRef]
- Vanangamudi, A.; Dumée, L.F.; Duke, M.C.; Yang, X. Nanofiber composite membrane with intrinsic janus surface for reversed-protein-fouling ultrafiltration. ACS Appl. Mater. Interfaces 2017, 9, 18328–18337. [Google Scholar] [CrossRef] [PubMed]
- Zhu, L.-P.; Yi, Z.; Liu, F.; Wei, X.-Z.; Zhu, B.-K.; Xu, Y.-Y. Amphiphilic graft copolymers based on ultrahigh molecular weight poly(styrene-alt-maleic anhydride) with poly(ethylene glycol) side chains for surface modification of polyethersulfone membranes. Eur. Polym. J. 2008, 44, 1907–1914. [Google Scholar] [CrossRef]
- Zhao, X.; He, C. Efficient preparation of super antifouling pvdf ultrafiltration membrane with one step fabricated zwitterionic surface. ACS Appl. Mater. Interfaces 2015, 7, 17947–17953. [Google Scholar] [CrossRef] [PubMed]
- Prince, J.A.; Bhuvana, S.; Anbharasi, V.; Ayyanar, N.; Boodhoo, K.V.K.; Singh, G. Self-cleaning metal organic framework (mof) based ultra filtration membranes—A solution to bio-fouling in membrane separation processes. Sci. Rep. 2014, 4. [Google Scholar] [CrossRef] [PubMed]
- Vanangamudi, A.; Saeki, D.; Dumée, L.F.; Duke, M.; Vasiljevic, T.; Matsuyama, H.; Yang, X. Surface-engineered biocatalytic composite membranes for reduced protein fouling and self-cleaning. ACS Appl. Mater. Interfaces 2018, 10, 27477–27487. [Google Scholar] [CrossRef] [PubMed]
- Chede, S.; Escobar, I.C. Fouling control using temperature responsive n-isopropylacrylamide (nipaam) membranes. Environ. Prog. Sustain. Energy 2016, 35, 416–427. [Google Scholar] [CrossRef]
- Rana, D.; Matsuura, T. Surface modifications for antifouling membranes. Chem. Rev. 2010, 110, 2448–2471. [Google Scholar] [CrossRef] [PubMed]
- Velicangil, O.; Howell, J.A. Self-cleaning membranes for ultrafiltration. Biotechnol. Bioeng. 1981, 23, 843–854. [Google Scholar] [CrossRef]
- Cordeiro, A.L.; Werner, C. Enzymes for antifouling strategies. J. Adhes. Sci. Technol. 2011, 25, 2317–2344. [Google Scholar] [CrossRef]
- Sun, L.; Liang, H.; Yuan, Q.; Wang, T.; Zhang, H. Study on a carboxyl-activated carrier and its properties for papain immobilization. J. Chem. Technol. Biotechnol. 2012, 87, 1083–1088. [Google Scholar] [CrossRef]
- Ansari, S.A.; Husain, Q. Potential applications of enzymes immobilized on/in nano materials: A review. Biotechnol. Adv. 2012, 30, 512–523. [Google Scholar] [CrossRef] [PubMed]
- Kim, J.; Grate, J.W.; Wang, P. Nanostructures for enzyme stabilization. Chem. Eng. Sci. 2006, 61, 1017–1026. [Google Scholar] [CrossRef]
- Wang, Z.-G.; Wan, L.-S.; Liu, Z.-M.; Huang, X.-J.; Xu, Z.-K. Enzyme immobilization on electrospun polymer nanofibers: An overview. J. Mol. Catal. B Enzym. 2009, 56, 189–195. [Google Scholar] [CrossRef]
- Al-Attabi, R.; Morsi, Y.; Schütz, J.A.; Dumée, L.F. One-pot synthesis of catalytic molybdenum based nanocomposite nano-fiber membranes for aerosol air remediation. Sci. Total Environ. 2019, 647, 725–733. [Google Scholar] [CrossRef] [PubMed]
- Al-Attabi, R.; Dumée, L.F.; Schütz, J.A.; Morsi, Y. Pore engineering towards highly efficient electrospun nanofibrous membranes for aerosol particle removal. Sci. Total Environ. 2018, 625, 706–715. [Google Scholar] [CrossRef] [PubMed]
- Vanangamudi, A.; Yang, X.; Duke, M.C.; Dumee, L.F. Nanofibers for membrane applications. In Handbook of Nanofibers; Barhoum, A., Bechelany, M., Makhlouf, A., Eds.; Springer: Cham, Switzerland, 2018. [Google Scholar]
- Jia, H.; Zhu, G.; Vugrinovich, B.; Kataphinan, W.; Reneker, D.H.; Wang, P. Enzyme-carrying polymeric nanofibers prepared via electrospinning for use as unique biocatalysts. Biotechnol. Prog. 2002, 18, 1027–1032. [Google Scholar] [CrossRef] [PubMed]
- Kim, T.G.; Park, T.G. Surface functionalized electrospun biodegradable nanofibers for immobilization of bioactive molecules. Biotechnol. Prog. 2006, 22, 1108–1113. [Google Scholar] [CrossRef] [PubMed]
- Srbová, J.; Slováková, M.; Křípalová, Z.; Žárská, M.; Špačková, M.; Stránská, D.; Bílková, Z. Covalent biofunctionalization of chitosan nanofibers with trypsin for high enzyme stability. React. Funct. Polym. 2016, 104, 38–44. [Google Scholar] [CrossRef]
- Silva, T.R.; Rodrigues, D.P.; Rocha, J.M.S.; Gil, M.H.; Pinto, S.C.S.; Lopes-da-Silva, J.A.; Guiomar, A.J. Immobilization of trypsin onto poly(ethylene terephthalate)/poly(lactic acid) nonwoven nanofiber mats. Biochem. Eng. J. 2015, 104, 48–56. [Google Scholar] [CrossRef]
- Ray, S.S.; Chen, S.-S.; Li, C.-W.; Nguyen, N.C.; Nguyen, H.T. A comprehensive review: Electrospinning technique for fabrication and surface modification of membranes for water treatment application. RSC Adv. 2016, 6, 85495–85514. [Google Scholar] [CrossRef]
- Schulze, A.; Breite, D.; Kim, Y.; Schmidt, M.; Thomas, I.; Went, M.; Fischer, K.; Prager, A. Bio-inspired polymer membrane surface cleaning. Polymers 2017, 9, 97. [Google Scholar] [CrossRef]
- Schulze, A.; Stoelzer, A.; Striegler, K.; Starke, S.; Prager, A. Biocatalytic self-cleaning polymer membranes. Polymers 2015, 7, 1837–1849. [Google Scholar] [CrossRef]
- Moreno-Cortez, I.E.; Romero-García, J.; González-González, V.; García-Gutierrez, D.I.; Garza-Navarro, M.A.; Cruz-Silva, R. Encapsulation and immobilization of papain in electrospun nanofibrous membranes of pva cross-linked with glutaraldehyde vapor. Mater. Sci. Eng. C 2015, 52, 306–314. [Google Scholar] [CrossRef] [PubMed]
- Tripathi, B.P.; Dubey, N.; Simon, F.; Stamm, M. Thermo responsive ultrafiltration membranes of grafted poly(n-isopropyl acrylamide) via polydopamine. RSC Adv. 2014, 4, 34073–34083. [Google Scholar] [CrossRef]
- Bae, Y.H.; Okano, T.; Kim, S.W. Temperature dependence of swelling of crosslinked poly(n,n′-alkyl substituted acrylamides) in water. J. Polym. Sci. Part B Polym. Phys. 1990, 28, 923–936. [Google Scholar] [CrossRef]
- Xu, Y.; Shi, L.; Ma, R.; Zhang, W.; An, Y.; Zhu, X.X. Synthesis and micellization of thermo- and ph-responsive block copolymer of poly(n-isopropylacrylamide)-block-poly(4-vinylpyridine). Polymer 2007, 48, 1711–1717. [Google Scholar] [CrossRef]
- Zhou, Q.; Li, J.-H.; Yan, B.-H.; Wu, D.; Zhang, Q.-Q. Thermo-responsive and antifouling PVDF nanocomposited membranes based on PNIPAAm modified TiO2 nanoparticles. Chin. J. Polym. Sci. 2014, 32, 892–905. [Google Scholar] [CrossRef]
- Guo, H.; Huang, J.; Wang, X. The alternate temperature-change cleaning behaviors of pnipaam grafted porous polyethylene membrane fouled by proteins. Desalination 2008, 234, 42–50. [Google Scholar] [CrossRef]
- Zhou, S.; Xue, A.; Zhang, Y.; Li, M.; Wang, J.; Zhao, Y.; Xing, W. Fabrication of temperature-responsive zro2 tubular membranes, grafted with poly (n-isopropylacrylamide) brush chains, for protein removal and easy cleaning. J. Membr. Sci. 2014, 450, 351–361. [Google Scholar] [CrossRef]
- Available online: http://www.worthington-biochem.com/TRY/default.html (accessed on 18 September 2018).
- Khaldi, M.; Blanpain-Avet, P.; Guérin, R.; Ronse, G.; Bouvier, L.; André, C.; Bornaz, S.; Croguennec, T.; Jeantet, R.; Delaplace, G. Effect of calcium content and flow regime on whey protein fouling and cleaning in a plate heat exchanger. J. Food Eng. 2015, 147, 68–78. [Google Scholar] [CrossRef]
- Jia, F.; Narasimhan, B.; Mallapragada, S. Materials-based strategies for multi-enzyme immobilization and co-localization: A review. Biotechnol. Bioeng. 2014, 111, 209–222. [Google Scholar] [CrossRef] [PubMed]
- Yu, J.-Z.; Zhu, L.-P.; Zhu, B.-K.; Xu, Y.-Y. Poly( n-isopropylacrylamide) grafted poly(vinylidene fluoride) copolymers for temperature-sensitive membranes. J. Membr. Sci. 2011, 366, 176–183. [Google Scholar] [CrossRef]
- Kang, K.; Kan, C.; Yeung, A.; Liu, D. The immobilization of trypsin on soap-free p(mma-ea-aa) latex particles. Mater. Sci. Eng. C 2006, 26, 664–669. [Google Scholar] [CrossRef]
- Zhang, K.; Wu, S.; Tang, X.; Kaiser, N.K.; Bruce, J.E. A bifunctional monolithic column for combined protein preconcentration and digestion for high throughput proteomics research. J. Chromatogr. B 2007, 849, 223–230. [Google Scholar] [CrossRef] [PubMed]
- Shimomura, M.; Ohta, M.; Sugiyama, N.; Oshima, K.; Yamauchi, T.; Miyauchi, S. Properties of α-chymotrypsin covalently immobilized on poly(acrylic acid)-grafted magnetite particles. Polym. J. 1999, 31, 274–278. [Google Scholar] [CrossRef]
Figure 1. Conceptual schematic of self-cleaning biocatalytic and thermo-switchable membrane.
Figure 2. SEM images of biocatalytic membranes with (a) no PNIPAAm (PN0-TR); (b) 2 wt % PNIPAAm (PN2-TR); and (c) 4 wt % PNIPAAm (PN4-TR).
Figure 3. Surface densities of TR immobilized on to PVDF/nylon-6,6/PNIPAAm membranes with no PNIPAAm (PN0-TR), 2 wt % (PN2-TR) and 4 wt % (PN4-TR) PNIPAAm concentrations.
Figure 4. Dynamic water contact angles (CAw) of the biocatalytic membranes with and without PNIPAAm for 60 s contact time at (a) 22 °C (Error bars are in the range 0.56−0.89°); (b) 50 °C (Error bars are in the range 0.45–1.2°); (c) differential pore number (in %) distributions (Error bars are in the range 0.2–0.6%); (d) enzymatic activities of biocatalytic membranes over time with no PNIPAAm, 2 and 4 wt % PNIPAAm.
Figure 5. Protein fouling studies for biocatalytic membranes with and without PNIPAAm. (a) Permeance values for two filtration cycles; (b) RPD after each filtration cycle; (c) PRR after each filtration cycle; (d) RF, IF and TF for 2 filtration cycles. Experimental Conditions: Pressure = 100 kPa, cross-flow velocity = 12.6 cm/s, feed solution = 1 g/L BSA, 1 mM CaCl2, 7 mM NaCl, both filtration and cleaning temperature = 22 °C.
Figure 6. SEM micrographs of BSA fouled biocatalytic membranes with (a) no PNIPAAm (PN0-TR); (b) 2 wt % (PN2-TR); and (c) 4 wt % (PN4-TR) PNIPAAm after two filtration and cleaning cycles at 22 °C.
Figure 7. Protein fouling studies for biocatalytic membranes with and without PNIPAAm. (a) Permeance values for two filtration cycles; (b) RPD after each filtration cycle (Error bars are in the range 1.1–2.9°). Experimental Conditions: Pressure = 100 kPa, cross-flow velocity = 12.6 cm/s, feed solution = 1 g/L BSA, 1 mM CaCl2, 7 mM NaCl, filtration temperature = 22 °C, cleaning temperature = 50 °C.
Figure 8. Hydrolytic activities of biocatalytic membranes for up to 14 days of storage at (a) 4 °C and (b) 22 °C; Stability of enzymes immobilized on to membranes in terms of enzyme activity with 50 °C treatment for 5 min after (c) one reuse cycle and (d) six reuse cycles.
© 2018 by the authors. Licensee MDPI, Basel, Switzerland. This article is an open access article distributed under the terms and conditions of the Creative Commons Attribution (CC BY) license (http://creativecommons.org/licenses/by/4.0/).