International Journal of Polymer Science

International Journal of Polymer Science / 2016 / Article

Research Article | Open Access

Volume 2016 |Article ID 7536397 |

Karol Fijałkowski, Rafał Rakoczy, Anna Żywicka, Radosław Drozd, Beata Zielińska, Karolina Wenelska, Krzysztof Cendrowski, Dorota Peitler, Marian Kordas, Maciej Konopacki, Ewa Mijowska, "Time Dependent Influence of Rotating Magnetic Field on Bacterial Cellulose", International Journal of Polymer Science, vol. 2016, Article ID 7536397, 13 pages, 2016.

Time Dependent Influence of Rotating Magnetic Field on Bacterial Cellulose

Academic Editor: Antje Potthast
Received15 Oct 2015
Revised15 Dec 2015
Accepted21 Dec 2015
Published18 Jan 2016


The aim of the study was to assess the influence of rotating magnetic field (RMF) on the morphology, physicochemical properties, and the water holding capacity of bacterial cellulose (BC) synthetized by Gluconacetobacter xylinus. The cultures of G. xylinus were exposed to RMF of frequency that equals 50 Hz and magnetic induction 34 mT for 3, 5, and 7 days during cultivation at 28°C in the customized RMF exposure system. It was revealed that BC exposed for 3 days to RMF exhibited the highest water retention capacity as compared to the samples exposed for 5 and 7 days. The observation was confirmed for both the control and RMF exposed BC. It was proved that the BC exposed samples showed up to 26% higher water retention capacity as compared to the control samples. These samples also required the highest temperature to release the water molecules. Such findings agreed with the observation via SEM examination which revealed that the structure of BC synthesized for 7 days was more compacted than the sample exposed to RMF for 3 days. Furthermore, the analysis of 2D correlation of Fourier transform infrared spectra demonstrated the impact of RMF exposure on the dynamics of BC microfibers crystallinity formation.

1. Introduction

Bacterial cellulose (BC) is an exopolysaccharide which can be produced by various species of bacteria; however only Gluconacetobacter xylinus has been considered as a model microorganism for its production and analysis [1]. The cellulose produced by G. xylinus exhibits high purity, high degree of crystallinity, high density, good shape retention, high water binding capacity, and higher surface area as compared to the plant cellulose [2, 3]. Due to these properties the BC has a wide range of potential applications including artificial skin [2, 4], dental implants [5], dialysis membrane [5, 6], coatings for cardiovascular stents [5], membranes for tissue-guided regeneration [2, 5], controlled-drug release carriers [5], vascular prosthetic devices [7], scaffolds for tissue engineering [2], wound dressing [5, 8, 9], and artificial blood vessels [10, 11]. Besides the applications in biomedical areas, BC membrane has also been used as separation medium for water treatment [12], carrier of battery fluids [13], viscosity modifier [4], biological substrate medium [14], or food or food substitute [4]. Additionally, a few new areas have been explored on developing the distinctive features of this novel biomaterial. The integration of the optical activity [15], electrical conductivity [16], magnetic nanoparticles [17], or photocatalytic degradation [18] materials to the BC matrix for various applications has also been studied.

In order to fulfill the requirements of diverse applications, the BC should be synthesized in the strictly defined culture conditions or subjected to different specific modifications [3]. It was previously shown that the biosynthesis of BC by microorganisms is directly influenced by the composition (nutrients nature) and conditions (static and dynamic) of culture medium, affecting BC yield, its macromorphology, and the arrangement of cellulose fibrils [19]. As reported by several authors, the BC obtained in the static culture conditions show enhanced arrangement of the BC fibril layer in comparison to the BC synthesized in dynamic culture conditions [20]. The latter one displays lower crystallinity, lower polymerization degree, and lower yield. Furthermore, it forms structure with high porosity and large water holding capacity [21]. It is also found that high oxygen content could disturb the arrangement process of the BC crystalline fibril structure [22].

The modification of BC can be performed during its biogenesis by the introduction of different substances into the BC-producing bacterium growth medium (hemicelluloses, cellulose derivatives, drugs, and dyes) or by modification of bacterial cells [23]. The modification affects, for example, the aggregation of nanofibers, crystallinity, crystallite size, polymerization, thermal stability, strength, porosity, roughness, morphology, and density [24]. The other approaches for modification of cellulose (plant or bacterial) include the use of physical factors, such as ultrasound irradiation (or sonication) [25, 26], static magnetic field (SMF) [2730], or rotating magnetic field (RMF) exposure [31].

The influence of the physical factors on the growth and cell metabolic activity can be attributed to its effects on mixing of the bioliquids at microlevels. The microscopic mixing can influence the transfer process between the cell surface and the liquid phase, affecting the cell transport mechanism [32]. Moreover, the RMF can cause relative motions of the medium and the magnetic flux lines [33]. The associated currents can be induced in the culture medium as a consequence of the magnetic field because the culture medium contains various cations, for example, Na+, K+, Mg2+, and NH4+, and the associated anions, for example, sulphate, phosphate, and chlorate, along with the microbial cells that contain various components including ionic solutions, proteins, and lipids. These factors are susceptible to the influence of magnetic or induced electric fields [33, 34]. Previous studies have also found that the cellulose nanocrystals have a negative diamagnetic anisotropy [35] and that they are oriented perpendicularly to the magnetic field direction [2729, 36]. Therefore, it was suggested that MFs may alter the cellulose nanocrystals orientation [37, 38].

In our previous study, we demonstrated that the constant exposure to the RMF for 3 days resulted in the cellulose yield characterized by higher water absorption, lower density, and less interassociated microfibrils comparing to the unexposed control [31]. However, it should be noticed that the stimulating effect of the RMF on the functional parameters of microorganisms was shown to be dependent on the time of magnetic field exposition [39, 40]. Similarly, the time of G. xylinus cultivation during which the BC biosynthesis occurs is considered as one of the crucial parameters affecting the properties of this material [22]. As reported by Hesse and Kondo [41] the cellulose secretion is randomly deposited behind the microorganism to produce the membrane of certain porosity and three-dimensional network. The movement of single cell is caused by the inverse force of the secretion of the cellulose nanofibers. Therefore, it can be assumed that the application of MF for different exposure time during the cellulose biosynthesis may influence the microstructure of the synthetized BC and thus its physical and chemical properties. Thus, in the current work, the effect of exposure time (3, 5, and 7 days) of the cellulose producing G. xylinus to RMF of frequency of 50 Hz and magnetic induction of 34 mT was assessed. The main purpose of this study was to examine whether a long-term (up to 7 days) exposure of G. xylinus to the RMF affects the morphology, physicochemical properties, and the water capacity of the synthetized cellulose. The obtained BC samples were analyzed using a set of analytical methods including Attenuated Total Reflectance Fourier Transform Infrared Spectroscopy (ATR-FTIR), X-ray diffraction (XRD) method, scanning electron microscopy (SEM), and dry/wet weight assessment and were compared to properties of cellulose produced in standard conditions (unexposed to RMF, the control).

2. Materials and Methods

2.1. BC Biosynthesis in RMF

The experiment was performed using the self-designed RMF exposure system adapted for the biological studies presented in Figure 1 and described in the previous work [31].

Briefly, the reference strain of G. xylinus (Deutsche Sammlung von Mikroorganismen und Zellkulturen, DSM 46604) was cultivated in the stationary conditions using a Hestrin-Schramm (HS) medium composed of glucose, 2 w/v%, yeast extract, 0.5 w/v%, bacto-peptone, 0.5 w/v%, citric acid, 0.115 w/v%, Na2HPO4, 0.27 w/v%, MgSO4·7H2O, 0.05 w/v%, bacteriological agar, 2% w/v, and ethanol, 1 v/v%, for 7 days at 28°C. Prior to the experiment, the 7-day culture was shaken and then 100 μL of the obtained bacterial suspension was used to inoculate 25 mL HS medium in 50 mL plastic tubes (3.8 cm diameter) (Polypropylene Conical Centrifuge Tube, Becton Dickinson and Company, USA) containing bacteria being exposed to the RMF. The frequency of the generated RMF and the magnetic induction was equal to 50 Hz and 34 mT, respectively. The magnetic exposure was carried out for 7 days at 28°C. The cellulose pellicles were collected in 3rd, 5th, and 7th day of the experiment. Each tube was used only once.

The same bacterial strain, incubated in the same time and under the same conditions but unexposed to the RMF, was generated as the control of experiment.

2.2. The Preparation of BC Samples

The BC was harvested from the medium and purified by the triplicate treatment with 0.1 M NaOH at 80°C for 30 min to remove the bacterial cells and medium components and then rinsed with water. The obtained cellulose was dried in an oven (EV-50, Trade Raypa, Spain) at 60°C until a constant weight was reached and investigated as described below.

2.3. Attenuated Total Reflectance Fourier Transform Infrared Spectroscopy (ATR-FTIR)

IR spectra of bacterial cellulose were performed by the ATR-FTIR method, using ALPHA FT-IR Spectrometer (Burker Co., Germany) with an DTGS detector and the platinum-ATR-sampling module with the robust diamond crystal and variable angle incidence of the beam. The measurements were carried out at an angle of 30°. The spectra were collected in the range of 4000–400 cm−1. For each of the samples 32 scans of the resolution of 2 cm−1 were performed. The spectra were collected and processed initially using the Omnic Software. The ATR-FTIR spectra of BC were analyzed by means of the two-dimensional correlation (2D correlation) analysis using 2Dshige software (Shigeaki Morita, Kwansei-Gakuin University, Nishinomiya, Japan). For the 2D correlation analysis, the areas of the spectra were restricted to the range between 1800 cm−1 and 650 cm−1, normalized at the frequency band of 660 cm−1 using the methodology described by Liu et al. [42, 43] and analyzed using Origin Pro 8 software.

The crystallinity index was calculated using the ratio of absorbance values for peaks 1430/900 (Cr.R1) and 1370/2900 (Cr.R2). The fraction of the cellulose was calculated from ATR-FTIR spectra according to the method described by Kataoka and Kondo [44]. The area of the peaks at 710 (710 cm−1) for and at 750 (750 cm−1) for was determined from the spectra deconvoluted in Peakfit software. The percentage of was calculated according to the formula:

2.4. X-Ray Diffraction (XRD)

The crystallographic structure of BC was evaluated by X-ray diffraction analysis (Philips, X’Pert PRO diffractometer). The CuKα radiation ( Å;  Å; 35 kV and 30 mA) was applied. The and were removed with the filter and the numerical procedure of Rachinger’s methods, respectively. The configuration of goniometer was Bragg-Brentano. The diffracted intensity of CuKα radiation was measured in a 2θ range between 5 and 35 with a step of 0.02. The Philips HighScore plus software was used for data evaluation. Moreover, the average size of the crystallites () was calculated using the Scherrer equation [45] based on the reflection of plane of 200:where is the line width originating solely from instrumental broadening; is the broadening of the diffraction line measured at half maximum intensity (FWHM); is shape factor (it is equal to 0.94) [45]; is X-ray wavelength (it is equal to 1.54 Å); is the Bragg angle corresponding to the (200) plane.

The shape factor 0.94 was assumed and broadening of the reflex originating solely from instrumental broadening and the size of the crystallites. The instrumental broadening was estimated by the measurement of silicon reference sample for several reflection and interpolation for 200 reflex.

2.5. Scanning Electron Microscopy (SEM)

The morphology of BC samples was investigated by scanning electron microscopy (TESCAN, VEGA SBU3). SEM images of as-prepared BC samples were acquired with 30 kV acceleration voltage.

2.6. Swelling Study

For the swelling study the cellulose pellicles were cut into 1 cm square samples and dried at 60°C for 6 h to remove any water content and weighed using analytical balance (accuracy 0.0001 g). Then samples were immersed in distilled water until a constant weight was reached (15 min). Afterwards, they were wiped carefully with filter paper and weighed again on the analytical balance. Each swelling experiment was taken in triplicate. The results are shown as percentage of swelling ratio (%SR) and calculated using the formula:

2.7. Water Holding Capacity

The cellulose pellicles were cut into small equal pieces, immersed in a distilled water for 15 min, wiped carefully with filter paper, and placed into the thermogravimetric analyzer (DTA-Q600 SDT TA). The analysis was performed in air flow (40 mL/min) from room temperature to 120°C, with the heating rate of 1°C/min. The results are shown as percentage of the sample weight loss versus the temperature. The initial weight of BC immersed in water was treated as 100%.

3. Results

3.1. Analysis of ATR-FTIR Spectra

The chemical structure of different BC samples was studied by ATR-FTIR. The spectrum shown in Figure 2 is characteristic absorption bands of BC functional groups indicating that the typical cellulose was produced [20].

In all the analyzed samples the bands that involve OH bending in the range of 400 to 700 cm−1 were found. The characteristic broad band present at ≈900 cm−1 corresponds to the beta glycosidic bond between the subunits of glucose. The presence of typical components of the glucose structure as (C-O, stretch) primary alcohols, antisymmetric out-of-phase stretching in pyranose ring, and C-O-C antisymmetric bridge stretching bands is confirmed in the range of 1058 to 1168 cm−1 indicated. The next region from 1200 to 1700 cm−1 corresponds to CH2 bending (≈1370 cm−1) and CH2 symmetric bending (≈1430 cm−1). The band at ≈1640 cm−1 indicates H-O-H bending of the absorbed water. The mode at 2900 cm−1 is related to the stretching of the CH2 and CH3 of the pyranose ring and the broad band at 3350 cm−1 is attributed to the OH stretching from intramolecular hydrogen bonds [46].

The analysis of the content of BC and crystalline phases showed similar amount of % allomorph form for both RMF exposed and the control BC (Table 1). The highest level of was recorded for BC samples synthesized for 5 days. It was also shown that the values of crystallinity indexes Cr.R1 and Cr.R2 calculated for the RMF exposed and control BC did not significantly vary in time.

Days of BC synthesisSampleCr.R1 1427/900Cr.R2 1360/2900%

3RMF exposed 3.143.0846.8

5RMF exposed 3.242.7749.8

7RMF exposed 3.383.2744.8

A synchronous 2D correlation spectrum exhibits the similarity between the sequential variations of the spectra intensities [47]. As reported by Noda [48], the 2D correlation analysis is suitable to establish the spectral band assignments but also to monitor the complex sequence of the events arising from the changes in the polymers. Furthermore, the 2D correlation method could be applied to understand the compositional and structural changes within the developed fibers in the presence of an external perturbation. A synchronous spectrum is a symmetric spectrum with respect to a diagonal line corresponding to the spectral coordinates [49]. The regions of a dynamic spectrum which change intensity to a greater extent are represented by the stronger autopeaks (diagonal peaks). The cross-peaks located at the off-diagonal positions of synchronous 2D correlation spectrum represent the simultaneous changes of the spectral signals at two different wave numbers [48].

Figure 3 shows the differences in the intensity of the bands pointing on the structural changes in BC occurring in the following days of the synthesis. The successive decrease in the intensity of the bands in the range from 1200 cm−1 to 800 cm−1 of the spectra region is related to the changes in structure and composition of the cellulose.

In the current study, the analysis of synchronous 2D correlation of ATR-FTIR spectra calculated from the time dependent ATR-FTIR spectra obtained from the region 850–1150 cm−1 was used to determine the BC maturity related to its microfibers crystallinity. The 2D correlations spectra are presented in Figures 4(a) and 4(b) for control BC and RMF exposed BC, respectively. As shown, RMF exposed samples were characterized by more dynamic changes in the range of analyzed spectra in comparison to the control BC. Two characteristic autopeaks at ≈968 cm−1 and ≈1042 cm−1 were observed on the diagonal of this plot, which indicate positive trend in altering their intensity. It might result from the presence of C-O stretching mode of primary alcohols (-C6H2-O6H), in which band at 968 cm−1 is characteristic for BC with a high degree of crystallinity, whereas the signal at 1042 cm−1 corresponds to the amorphous form of cellulose. The analyzed spectra showed also the intense cross-peaks observed outside the diagonal axis referring to the above-mentioned signals and indicating that there have been changes in crystallinity in these regions [43].

3.2. X-Ray Diffraction Analyses

The XRD patterns of the BC synthesized in the control conditions and under RMF exposure are presented in Figure 5. From this figure it is clearly seen that XRD patterns of all studied samples exhibited three diffraction peaks at 2θ value of around 14.6°, 16.8°, and 22.8°. All those reflections are assigned to the cellulose phase (JCPDS card number 50-2241) and correspond to the diffraction planes of (1–10), (110), and (200), respectively [50].

The average crystallite size calculated for the synthesized samples is shown in Table 2. It can be seen that the crystallites size was not significantly changed when BC was synthesized in the presence of RMF. Additionally, the time dependence versus the crystallite size for both control and RMF exposed samples has been detected. The longer growth time induced the reduction of the crystallites size.

SampleDays of BC synthesisAverage crystallite size [nm]

RMF exposed38.4
RMF exposed56.7
RMF exposed76.4

3.3. Structure of Bacterial Cellulose

The SEM micrographs showing the BC structure are presented in Figure 6. From the comparison of the BC fibers orientation, significant differences in the samples incubated for longer period were revealed. It was shown that the structure of the cellulose after 5 and 7 days was more compacted (dense), in the case of both RMF exposed and control BC, in comparison to the respective samples produced in 3 days. It was also observed that application of the RMF during BC synthesis resulted in the long fiber formation. This effect was enhanced in the sample after 3 days of the culture under RMF influence (Figure 7). The difference between the length of the fibers after further time extension is less noticeable due to the high structure density and entanglement of the fibers. However, it is not excluded that the longer fibers are also present in the samples after 5 and 7 days of growth. They exhibit similar structure of high density with long, tangled fibers.

3.4. Swelling and Water Retention Characteristics

The cellulose obtained in the RMF was characterized by higher ability to swell by water accumulation as compared to the cellulose obtained under the standard conditions (Figure 8). It was also recorded that swelling properties of BC decreased with time in the similar manner for both control BC and BC from RMF exposed cultures. The difference between the swelling ratio calculated for the BC obtained from different culture conditions was 26%, 18%, and 16% for BC synthesized for 3, 5, and 7 days, respectively.

In order to study the water holding capacity of the samples in great detail, TGA analysis was performed from room temperature to 120°C. The control BC exhibited 94%, 98%, and 100% of the weight loss for the samples prepared in 3, 5, and 7 days, respectively (Figure 9(a)). In the case of the BC samples produced in the presence of RMF, the percentage of sample weight loss was 87%, 89%, and 99%, for 3, 5, and 7 days, correspondingly (Figure 9(b)).

4. Discussion

Currently, there is abundant evidence that various types of MFs affect the functional processes of the microorganisms and influence their biotechnological potential [51]. The studies on the use of MFs in the biotechnological process conducted to date have concerned mostly the SMF, whereas the RMF still remains unexplored [31, 52]. However, their effects on microorganisms and substances produced by them can differ due to the different nature of the SMF and the RMF. It should be noticed that the SMF does not vary over time or changes slowly and does not have frequency [53]. In contrast, the RMF changes over time and can be characterized by its frequency [54]. The effect of the magnetic stimulation on bacteria depends on the magnetic frequency, the magnetic induction, and the time of exposure. In previous studies we proved that the exposure to the RMF depended on those parameters and influenced growth and metabolic activity of the different microorganisms [39, 40].

Biocellulose produced by G. xylinus contains more than 90% of water [55]. The water resides inside the BC pores and is bound to the cellulose fibrils through hydrogen bonding [56]. The swelling in water capacity and water release rate are considered the most important properties which are directly involved in the biomedical applications of BC as a dressing material [57]. Both parameters have a direct relation with the BC fibril arrangement [57]. The BC microstructure, in turn, determines the usefulness of this material as carrier supports for the immobilization of microorganisms and proteins [58, 59]. The current study revealed that the cellulose obtained under RMF influences both water absorption and density of microfibrils. However, these effects strictly depended on the synthesis time and exposure to RMF time.

Gretz et al. [60] demonstrated that magnetically altered BC was characterized by the greater capacity of water absorption, greater chemical reactivity, lower density, lower tensile strength, and greater surface area. These authors suggested that the altered cellulose produced by G. xylinus is a result of direct magnetic interaction with β-glucan during its crystallization. Previous studies have also revealed that cellulose nanocrystals have a negative diamagnetic anisotropy [35] and that they are oriented perpendicularly to the magnetic field [2730]. Therefore, it was suggested that MFs may be applied to control the cellulose nanocrystals orientation and its influence on BC cellulose fibrils crystal network formation rate [37, 38]. In this study, changes in the intensity of the ATR-FTIR spectra in the region from 900 cm−1 to 1150 cm−1 (2D spectra) were characterized by higher dynamics in the case of the BC samples from the cultures exposed to RMF. This may suggest that higher intensity of the changes in the molecular structure of cellulose may have an impact on the rate of its microfibrils crystallization. Unfortunately, due to the complexity of this process, it is difficult to determine unequivocally which factor is crucial. BC synthesis process consists of two stages, polymerization and crystallization. The polymerization step is catalyzed by the cellulose synthase complex. After extraction of the polyglucan outside of the bacterial cell, the association of the chains and the formation of the cellulose microfibril crystalline structure occurs. The stabilization of the highly ordered BC structure is dependent on the hydrophobic interactions and hydrogen bonds formed between hydroxyl groups of neighboring β-glucan chains [61, 62]. Recent studies have indicated an important role of water molecules in the process of cellulose crystalline structure formation. It can be assumed that water can be involved in the formation of the crystal structure of cellulose, facilitating (catalyzing) the alignment of β-glucans chains through hydrogen-bonded bridging [63]. In this case, RMF may have a significant impact on the formation of hydrogen-bonded bridging. Previous studies have confirmed the influence of SMF on physicochemical properties of water. It was shown that SMF can reduce the surface tension of water and increase its viscosity. The disorder in the ability of water molecules to form hydrogen bonds stabilizes its crystal structure [6466]. These changes are likely to have an impact on the rate of BC crystalline structure formation and its quality. The observation from the SEM examination revealed that the structure of the cellulose after 5 and 7 days was more compacted (dense), in case of both RMF exposed and control BC, in comparison to the respective samples produced in 3 days. Cellulose chains forming subelementary fibrils are extruded out of the surface of the bacterial cell into the culture medium. These subfibrils aggregate together forming larger microfibrils [67]. Therefore the density of BC increases with culture time due to the secretion of more fibrils with the passage of time [68]. It was also observed that application of the RMF during BC synthesis resulted in the long fiber formation and consequently more tangled and compacted fibrous structure. This effect was especially clearly seen after 3 days of culture under RMF influence (long fiber appearance) and after 5 days with and without RMF exposure (higher density). The observed changes in the morphology of the samples can be responsible for the water swelling and water holding properties observed for cellulose from RMF exposed cultures. In the present study, the BC obtained after 3 days presented the most interesting behavior of water absorption. The observation was confirmed for both control and RMF exposed BC and obviously it was mainly related to the loose structure of young cellulose matrix. However, the cellulose obtained in the presence of RMF showed 26% higher ability to swell in water in comparison to the control cellulose. Similar results were obtained in our previous studies [31], in which, as a result of exposure of G. xylinus cultures to RMF during 3 days cultivation, the obtained BC was characterized by increased water absorption by 23% as compared to the unexposed control sample. Our observation also agreed with the previous results reported by Al-Shamary and Al-Darwash [69] in which the density of BC increased during the cultivation, whereas water capacity decreased due to the increased secretion of the fibrils with time. However, it should be noticed that, in the case of our study, cellulose synthetized for 7 days in RMF was still characterized by significantly higher water adsorption capacity (16%) as compared to the unexposed control polymer. Moreover, from a comparison of the current and the previous studies, which involved the use of different G. xylinus strains, it can be concluded that the effect caused by magnetic field seems to be independent of the particular strain. However, this assumption should be further confirmed with a larger number of different G. xylinus strains.

The high ability to swell in water of BC could arise from differences in the material microstructure due to the different culture conditions and time of exposure to RMF. The water absorption capacity depends especially on the number and size of pores on the polymer surface. It was reported by several authors that the loose fibril arrangement and large size of pores enhance the water capacity of BC [70, 71]. It is considered that closely arranged microfibrils bind the water molecules more efficiently due to the stronger hydrogen bonding interactions, as compared to the loosely arranged microfibrils [72, 73]. Furthermore, it was demonstrated that more water can be retained due to the larger surface area provided by thinner and longer fibers [74]. In the present study, it was also shown that RMF exposed BC released water slightly slower and required the highest temperature to release water molecules as compared to the unexposed controls. This observation is particularly surprising considering looser structure of these BC samples. In this case, increased ability to retain water might be explained by the size of pores in the investigated BC samples. It was reported by Ul-Islam et al. [57] that cellulose membranes with smaller pore sizes can retain water in the matrix for longer times. Although the porosity of BC was not examined in our study, it can be assumed that the exposure to the RMF might result in formation of smaller pores in these samples, protecting the water from evaporation.

5. Conclusions

Summarizing, the current study intends to produce BC with altered morphology, physicochemical properties, the water retention and holding capacity synthesized in G. xylinus cultures exposed to the RMF of 50 Hz frequency, and magnetic induction of 34 mT for 3, 5, and 7 days. It was observed by SEM that application of the RMF during BC synthesis influenced its nano- and microscale structure. The RMF altered cellulose, regardless of the synthesis time, was characterized by significantly higher water adsorption capacity as compared to unexposed control samples. The physicochemical properties of BC studied by ATR-FTIR and XRD were similar regardless of the culture conditions employed. The only differences found in the synchronous 2D correlation of ATR-FTIR spectra indicated the impact of RMF exposure on the dynamics of the formation of BC microfibers crystallinity. Therefore it can be concluded that the impact of the RMF which allows improving the useful properties of water behavior in BC while not compromising the remaining properties of the polymer may provide a novel technique for altering cellulose biogenesis and when fully developed may find application in the multiple biotechnological applications.

Conflict of Interests

The authors declare that there is no conflict of interests regarding the publication of this paper.


This study was supported by the National Centre for Research and Development in Poland (Grant no. LIDER/011/221/L-5/13/NCBR/2014).


  1. D. Mikkelsen, B. M. Flanagan, G. A. Dykes, and M. J. Gidley, “Influence of different carbon sources on bacterial cellulose production by Gluconacetobacter xylinus strain ATCC 53524,” Journal of Applied Microbiology, vol. 107, no. 2, pp. 576–583, 2009. View at: Publisher Site | Google Scholar
  2. W. K. Czaja, D. J. Young, M. Kawecki, and R. M. Brown Jr., “The future prospects of microbial cellulose in biomedical applications,” Biomacromolecules, vol. 8, no. 1, pp. 1–12, 2007. View at: Publisher Site | Google Scholar
  3. D. R. Ruka, G. P. Simon, and K. M. Dean, “Altering the growth conditions of Gluconacetobacter xylinus to maximize the yield of bacterial cellulose,” Carbohydrate Polymers, vol. 89, no. 2, pp. 613–622, 2012. View at: Publisher Site | Google Scholar
  4. R. Jonas and L. F. Farah, “Production and application of microbial cellulose,” Polymer Degradation and Stability, vol. 59, no. 1–3, pp. 101–106, 1998. View at: Publisher Site | Google Scholar
  5. W. K. Wan and L. E. Millon, “Poly(vinyl alcohol)-bacterial cellulose nanocomposite,” US Patent Applications, US 2005037082 A1 16, 2005. View at: Google Scholar
  6. A. M. Sokolnicki, R. J. Fisher, T. P. Harrah, and D. L. Kaplan, “Permeability of bacterial cellulose membranes,” Journal of Membrane Science, vol. 272, no. 1-2, pp. 15–27, 2006. View at: Publisher Site | Google Scholar
  7. P. A. Charpentier, A. Maguire, and W.-K. Wan, “Surface modification of polyester to produce a bacterial cellulose-based vascular prosthetic device,” Applied Surface Science, vol. 252, no. 18, pp. 6360–6367, 2006. View at: Publisher Site | Google Scholar
  8. V. I. Legeza, V. P. Galenko-Yaroshevskii, E. V. Zinov'ev et al., “Effects of new wound dressings on healing of thermal burns of the skin in acute radiation disease,” Bulletin of Experimental Biology and Medicine, vol. 138, no. 3, pp. 311–315, 2004. View at: Publisher Site | Google Scholar
  9. W. Czaja, A. Krystynowicz, S. Bielecki, and R. M. Brown Jr., “Microbial cellulose—the natural power to heal wounds,” Biomaterials, vol. 27, no. 2, pp. 145–151, 2006. View at: Publisher Site | Google Scholar
  10. H. Bäckdahl, G. Helenius, A. Bodin et al., “Mechanical properties of bacterial cellulose and interactions with smooth muscle cells,” Biomaterials, vol. 27, no. 9, pp. 2141–2149, 2006. View at: Publisher Site | Google Scholar
  11. W. K. Wan, J. L. Hutter, L. Milion, and G. Guhados, “Bacterial cellulose and its nanocomposites for biomedical applications,” ACS Symposium Series, vol. 938, pp. 221–241, 2006. View at: Publisher Site | Google Scholar
  12. Y.-J. Choi, Y. Ahn, M.-S. Kang, H.-K. Jun, I. S. Kim, and S.-H. Moon, “Preparation and characterization of acrylic acid-treated bacterial cellulose cation-exchange membrane,” Journal of Chemical Technology and Biotechnology, vol. 79, no. 1, pp. 79–84, 2004. View at: Publisher Site | Google Scholar
  13. R. M. Brown, “Microbial cellulose as a building block resource for specialty products and processes therefore,” PCT International Applications, WO 8912107 A1 (1989) 37, 1993. View at: Google Scholar
  14. K. Watanabe, Y. Eto, S. Takano, S. Nakamori, H. Shibai, and S. Yamanaka, “A new bacterial cellulose substrate for mammalian cell culture,” Cytotechnology, vol. 13, no. 2, pp. 107–114, 1993. View at: Publisher Site | Google Scholar
  15. W. Hu, S. Liu, S. Chen, and H. Wang, “Preparation and properties of photochromic bacterial cellulose nanofibrous membranes,” Cellulose, vol. 18, no. 3, pp. 655–661, 2011. View at: Publisher Site | Google Scholar
  16. W. Hu, S. Chen, Z. Yang, L. Liu, and H. Wang, “Flexible electrically conductive nanocomposite membrane based on bacterial cellulose and polyaniline,” Journal of Physical Chemistry B, vol. 115, no. 26, pp. 8453–8457, 2011. View at: Publisher Site | Google Scholar
  17. W. Zhang, S. Chen, W. Hu et al., “Facile fabrication of flexible magnetic nanohybrid membrane with amphiphobic surface based on bacterial cellulose,” Carbohydrate Polymers, vol. 86, no. 4, pp. 1760–1767, 2011. View at: Publisher Site | Google Scholar
  18. X. Zhang, W. Chen, Z. Lin, and J. Shen, “Photocatalytic degradation of a methyl orange wastewater solution using titanium dioxide loaded on bacterial cellulose,” Synthesis and Reactivity in Inorganic, Metal-Organic and Nano-Metal Chemistry, vol. 41, no. 9, pp. 1141–1147, 2011. View at: Publisher Site | Google Scholar
  19. K.-Y. Lee, G. Buldum, A. Mantalaris, and A. Bismarck, “More than meets the eye in bacterial cellulose: biosynthesis, bioprocessing, and applications in advanced fiber composites,” Macromolecular Bioscience, vol. 14, no. 1, pp. 10–32, 2014. View at: Publisher Site | Google Scholar
  20. W. Czaja, D. Romanovicz, and R. m. Brown,, “Structural investigations of microbial cellulose produced in stationary and agitated culture,” Cellulose, vol. 11, no. 3, pp. 403–411, 2004. View at: Publisher Site | Google Scholar
  21. N. Suwannapinunt, J. Burakorn, and S. Thaenthanee, “Effect of culture conditions on bacterial cellulose (BC) production from Acetobacter xylinum TISTR976 and physical properties of BC parchment paper,” Suranaree Journal of Science and Technology, vol. 14, no. 4, pp. 357–365, 2007. View at: Google Scholar
  22. M. Hornung, M. Ludwig, A. M. Gerrard, and H.-P. Schmauder, “Optimizing the production of bacterial cellulose in surface culture: evaluation of substrate mass transfer influences on the bioreaction (part 1),” Engineering in Life Sciences, vol. 6, no. 6, pp. 537–545, 2006. View at: Publisher Site | Google Scholar
  23. M. Seifert, S. Hesse, V. Kabrelian, and D. Klemm, “Controlling the water content of never dried and reswollen bacterial cellulose by the addition of water-soluble polymers to the culture medium,” Journal of Polymer Science, Part A: Polymer Chemistry, vol. 42, no. 3, pp. 463–470, 2004. View at: Publisher Site | Google Scholar
  24. Z. Yan, S. Chen, H. Wang, B. Wang, and J. Jiang, “Biosynthesis of bacterial cellulose/multi-walled carbon nanotubes in agitated culture,” Carbohydrate Polymers, vol. 74, no. 3, pp. 659–665, 2008. View at: Publisher Site | Google Scholar
  25. S.-S. Wong, S. Kasapis, and Y. M. Tan, “Bacterial and plant cellulose modification using ultrasound irradiation,” Carbohydrate Polymers, vol. 77, no. 2, pp. 280–287, 2009. View at: Publisher Site | Google Scholar
  26. S.-S. Wong, S. Kasapis, and D. Huang, “Molecular weight and crystallinity alteration of cellulose via prolonged ultrasound fragmentation,” Food Hydrocolloids, vol. 26, no. 2, pp. 365–369, 2012. View at: Publisher Site | Google Scholar
  27. J. Sugiyama, H. Chanzy, and G. Maret, “Orientation of cellulose microcrystals by strong magnetic fields,” Macromolecules, vol. 25, no. 16, pp. 4232–4234, 1992. View at: Publisher Site | Google Scholar
  28. P. G. de Gennes and J. Prost, The Physics of Liquid Crystals, Clarendon Press, Oxford, UK, 1993.
  29. J. F. Revol, L. Godbout, X.-M. Dong, D. G. Gray, H. Chanzy, and G. Maret, “Chiral nematic suspensions of cellulose crystallites; phase separation and magnetic field orientation,” Liquid Crystals, vol. 16, no. 1, pp. 127–134, 1994. View at: Publisher Site | Google Scholar
  30. F. Kimura, T. Kimura, M. Tamura, A. Hirai, M. Ikuno, and F. Horii, “Magnetic alignment of the chiral nematic phase of a cellulose microfibril suspension,” Langmuir, vol. 21, no. 5, pp. 2034–2037, 2005. View at: Publisher Site | Google Scholar
  31. K. Fijałkowski, A. Żywicka, R. Drozd et al., “Modification of bacterial cellulose through exposure to the rotating magnetic field,” Carbohydrate Polymers, vol. 133, pp. 52–60, 2015. View at: Publisher Site | Google Scholar
  32. R. W. Hunt, A. Zavalin, A. Bhatnagar, S. Chinnasamy, and K. C. Das, “Electromagnetic biostimulation of living cultures for biotechnology, biofuel and bioenergy applications,” International Journal of Molecular Sciences, vol. 10, no. 10, pp. 4515–4558, 2009. View at: Publisher Site | Google Scholar
  33. E. S. A. Gaafar, M. S. Hanafy, E. Y. Tohamy, and M. H. Ibranhim, “The effect of electromagnetic field on protein molecular structure of E. coli and its pathogenesis,” Romanian Journal of Biophysics, vol. 18, no. 2, pp. 145–169, 2008. View at: Google Scholar
  34. V. Anton-Leberre, E. Haanappel, N. Marsaud et al., “Exposure to high static or pulsed magnetic fields does not affect cellular processes in the yeast Saccharomyces cerevisiae,” Bioelectromagnetics, vol. 31, no. 1, pp. 28–38, 2010. View at: Publisher Site | Google Scholar
  35. E. D. Cranston and D. G. Gray, “Formation of cellulose-based electrostatic layer-by-layer films in a magnetic field,” Science and Technology of Advanced Materials, vol. 7, no. 4, pp. 319–321, 2006. View at: Publisher Site | Google Scholar
  36. T. Kimura, T. Kamioka, and S. Kuga, “Filtration-assisted magnetic micropatterning of bacterial cellulose,” Polymer Journal, vol. 39, no. 11, pp. 1199–1201, 2007. View at: Publisher Site | Google Scholar
  37. M. Park, S. Park, and J. Hyun, “Use of magnetic nanoparticles to manipulate the metabolic environment of bacteria for controlled biopolymer synthesis,” ACS Applied Materials and Interfaces, vol. 4, no. 10, pp. 5114–5117, 2012. View at: Publisher Site | Google Scholar
  38. J. P. F. Lagerwall, C. Schütz, M. Salajkova et al., “Cellulose nanocrystal-based materials: from liquid crystal self-assembly and glass formation to multifunctional thin films,” NPG Asia Materials, vol. 6, article e80, 2014. View at: Publisher Site | Google Scholar
  39. K. Fijałkowski, P. Nawrotek, M. Struk, M. Kordas, and R. Rakocz, “The effects of rotating magnetic field on growth rate, cell metabolic activity and biofilm formation by Staphylococcus aureus and Escherichia coli,” Journal of Magnetics, vol. 18, no. 3, pp. 289–296, 2013. View at: Publisher Site | Google Scholar
  40. P. Nawrotek, K. Fijałkowski, M. Struk, M. Kordas, and R. Rakoczy, “Effects of 50 Hz rotating magnetic field on the viability of Escherichia coli and Staphylococcus aureus,” Electromagnetic Biology and Medicine, vol. 33, no. 1, pp. 29–34, 2014. View at: Publisher Site | Google Scholar
  41. S. Hesse and T. Kondo, “Behavior of cellulose production of Acetobacter xylinum in 13C-enriched cultivation media including movements on nematic ordered cellulose templates,” Carbohydrate Polymers, vol. 60, no. 4, pp. 457–465, 2005. View at: Publisher Site | Google Scholar
  42. Y. Liu, G. Gamble, and D. Thibodeaux, “Two-dimensional attenuated total reflection infrared correlation spectroscopy study of the desorption process of water-soaked cotton fibers,” Applied Spectroscopy, vol. 64, no. 12, pp. 1355–1363, 2010. View at: Publisher Site | Google Scholar
  43. Y. Liu, D. Thibodeaux, G. Gamble, P. Bauer, and D. VanDerveer, “Comparative investigation of fourier transform infrared (FT-IR) spectroscopy and X-ray diffraction (XRD) in the determination of cotton fiber crystallinity,” Applied Spectroscopy, vol. 66, no. 8, pp. 983–986, 2012. View at: Publisher Site | Google Scholar
  44. Y. Kataoka and T. Kondo, “Quantitative analysis for the cellulose Iα crystalline phase in developing wood cell walls,” International Journal of Biological Macromolecules, vol. 24, no. 1, pp. 37–41, 1999. View at: Publisher Site | Google Scholar
  45. M. Poletto, H. L. Ornaghi Jr., and A. J. Zattera, “Native cellulose: structure, characterization and thermal properties,” Materials, vol. 7, no. 9, pp. 6105–6119, 2014. View at: Publisher Site | Google Scholar
  46. R. H. Atalla, “Celluloses,” in Carbohydrates and Their Derivatives Including Tannins, Cellulose, and Related Lignings, B. M. Pinto, Ed., vol. 3 of Comprehensive Natural Products Chemistry, pp. 529–598, Elsevier, Amsterdam, The Netherlands, 1999. View at: Google Scholar
  47. Y. Park, I. Noda, and Y. M. Jung, “Two-dimensional correlation spectroscopy in polymer study,” Frontiers in Chemistry, vol. 3, article 14, 2015. View at: Publisher Site | Google Scholar
  48. I. Noda, “Generalized two-dimensional correlation method applicable to infrared, Raman, and other types of spectroscopy,” Applied Spectroscopy, vol. 47, no. 9, pp. 1329–1336, 1993. View at: Publisher Site | Google Scholar
  49. V. G. Gregoriou and M. S. Braiman, Vibrational Spectroscopy of Biological and Polymeric Materials, CRC Press, Taylor & Francis Group, Boca Raton, Fla, USA, 2006.
  50. J.-H. Pang, X. Liu, M. Wu, Y.-Y. Wu, X.-M. Zhang, and R.-C. Sun, “Fabrication and characterization of regenerated cellulose films using different ionic liquids,” Journal of Spectroscopy, vol. 2014, Article ID 214057, 8 pages, 2014. View at: Publisher Site | Google Scholar
  51. L. Fojt, L. Strašák, V. Vetterl, and J. Šmarda, “Comparison of the low-frequency magnetic field effects on bacteria Escherichia coli, Leclercia adecarboxylata and Staphylococcus aureus,” Bioelectrochemistry, vol. 63, no. 1-2, pp. 337–341, 2004. View at: Publisher Site | Google Scholar
  52. J. Hristov, “Magnetic field assisted fluidization—a unified approach. Part 8. Mass transfer: magnetically assisted bioprocesses,” Reviews in Chemical Engineering, vol. 26, no. 3-4, pp. 55–128, 2010. View at: Publisher Site | Google Scholar
  53. S. Shanmugapriya, A. Sarumathi, and N. Saravanan, “Study of lipid profile changes and histopathology examination of heart under immobilization stress with static magnetic field exposure in rats,” International Journal of Environmental Biology, vol. 2, pp. 41–49, 2012. View at: Google Scholar
  54. R. Rakoczy, “Mixing energy investigations in a liquid vessel that is mixed by using a rotating magnetic field,” Chemical Engineering and Processing: Process Intensification, vol. 66, pp. 1–11, 2013. View at: Publisher Site | Google Scholar
  55. N. Pa'E, N. I. A. Hamid, N. Khairuddin et al., “Effect of different drying methods on the morphology, crystallinity, swelling ability and tensile properties of nata de coco,” Sains Malaysiana, vol. 43, no. 5, pp. 767–773, 2014. View at: Google Scholar
  56. K. Gelin, A. Bodin, P. Gatenholm, A. Mihranyan, K. Edwards, and M. Strømme, “Characterization of water in bacterial cellulose using dielectric spectroscopy and electron microscopy,” Polymer, vol. 48, no. 26, pp. 7623–7631, 2007. View at: Publisher Site | Google Scholar
  57. M. Ul-Islam, T. Khan, and J. K. Park, “Water holding and release properties of bacterial cellulose obtained by in situ and ex situ modification,” Carbohydrate Polymers, vol. 88, no. 2, pp. 596–603, 2012. View at: Publisher Site | Google Scholar
  58. S.-C. Wu and Y.-K. Lia, “Application of bacterial cellulose pellets in enzyme immobilization,” Journal of Molecular Catalysis B: Enzymatic, vol. 54, no. 3-4, pp. 103–108, 2008. View at: Publisher Site | Google Scholar
  59. N. M. N. Ton, M. D. Nguyen, T. T. H. Pham, and V. V. M. Le, “Influence of initial pH and sulfur dioxide content in must on wine fermentation by immobilized yeast in bacterial cellulose,” International Food Research Journal, vol. 17, no. 3, pp. 743–749, 2010. View at: Google Scholar
  60. M. R. Gretz, D. B. Folsom, and R. M. Brown Jr., “Cellulose biogenesis in bacteria and higher plants is disrupted by magnetic fields,” Naturwissenschaften, vol. 76, no. 8, pp. 380–383, 1989. View at: Publisher Site | Google Scholar
  61. M. Benziman, C. H. Haigler, and R. M. Brown Jr., “Cellulose biogenesis: polymerization and crystallization are coupled processes in Acetobacter xylinum,” Proceedings of the National Academy of Sciences of the United States of America, vol. 77, no. 11, pp. 6678–6682, 1980. View at: Publisher Site | Google Scholar
  62. J. L. W. Morgan, J. Strumillo, and J. Zimmer, “Crystallographic snapshot of cellulose synthesis and membrane translocation,” Nature, vol. 493, no. 7431, pp. 181–186, 2013. View at: Publisher Site | Google Scholar
  63. D. P. Shelton, “Long-range orientation correlation in water,” The Journal of Chemical Physics, vol. 141, no. 22, Article ID 224506, 2014. View at: Publisher Site | Google Scholar
  64. X.-F. Pang and D. Bo, “The changes of macroscopic features and microscopic structures of water under influence of magnetic field,” Physica B: Condensed Matter, vol. 403, no. 19-20, pp. 3571–3577, 2008. View at: Publisher Site | Google Scholar
  65. A. Szcześ, E. Chibowski, L. Hołysz, and P. Rafalski, “Effects of static magnetic field on water at kinetic condition,” Chemical Engineering and Processing: Process Intensification, vol. 50, no. 1, pp. 124–127, 2011. View at: Publisher Site | Google Scholar
  66. E. J. L. Toledo, T. C. Ramalho, and Z. M. Magriotis, “Influence of magnetic field on physical-chemical properties of the liquid water: insights from experimental and theoretical models,” Journal of Molecular Structure, vol. 888, no. 1–3, pp. 409–415, 2008. View at: Publisher Site | Google Scholar
  67. F. Horii, H. Yamamoto, and A. Hirai, “Microstructural analysis of microfibrils of bacterial cellulose,” Macromolecular Symposia, vol. 120, pp. 197–205, 1997. View at: Publisher Site | Google Scholar
  68. W. Tang, S. Jia, Y. Jia, and H. Yang, “The influence of fermentation conditions and post-treatment methods on porosity of bacterial cellulose membrane,” World Journal of Microbiology and Biotechnology, vol. 26, no. 1, pp. 125–131, 2010. View at: Publisher Site | Google Scholar
  69. E. E. Al-Shamary and A. K. Al-Darwash, “Influence of fermentation condition and alkali treatment on the porosity and thickness of bacterial cellulose membranes,” The Online Journal of Science and Technology, vol. 3, no. 2, 2013. View at: Google Scholar
  70. Y. Dahman, “Nanostructured biomaterials and biocomposites from bacterial Cellulose nanofibers,” Journal of Nanoscience and Nanotechnology, vol. 9, no. 9, pp. 5105–5122, 2009. View at: Publisher Site | Google Scholar
  71. J. Guo and J. M. Catchmark, “Surface area and porosity of acid hydrolyzed cellulose nanowhiskers and cellulose produced by Gluconacetobacter xylinus,” Carbohydrate Polymers, vol. 87, no. 2, pp. 1026–1037, 2012. View at: Publisher Site | Google Scholar
  72. H. Ougiya, K. Watanabe, T. Matsumura, and F. Yoshinaga, “Relationship between suspension properties and fibril structure of disintegrated bacterial cellulose,” Bioscience, Biotechnology and Biochemistry, vol. 62, no. 9, pp. 1714–1719, 1998. View at: Publisher Site | Google Scholar
  73. N. Shah, J. H. Ha, and J. K. Park, “Effect of reactor surface on production of bacterial cellulose and water soluble oligosaccharides by Gluconacetobacter hansenii PJK,” Biotechnology and Bioprocess Engineering, vol. 15, no. 1, pp. 110–118, 2010. View at: Publisher Site | Google Scholar
  74. B. V. Mohite and S. V. Patil, “Physical, structural, mechanical and thermal characterization of bacterial cellulose by G. hansenii NCIM 2529,” Carbohydrate Polymers, vol. 106, no. 1, pp. 132–141, 2014. View at: Publisher Site | Google Scholar

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