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Surface deposited one-dimensional copper-doped TiO2 nanomaterials for prevention of health care acquired infections

  • Tilen Koklic,

    Roles Conceptualization, Data curation, Formal analysis, Supervision, Writing – original draft, Writing – review & editing

    Affiliations Department of Condensed Matter Physics, Jožef Stefan Institute, Ljubljana, Slovenia, NAMASTE Center of Excellence, Ljubljana, Slovenia

  • Iztok Urbančič,

    Roles Investigation, Methodology, Software, Writing – original draft

    Affiliations Department of Condensed Matter Physics, Jožef Stefan Institute, Ljubljana, Slovenia, University of Oxford, John Radcliffe Hospital, The Weatherall Institute of Molecular Medicine, Human Immunology Unit, Headington, Oxford, United Kingdom

  • Irena Zdovc,

    Roles Investigation, Methodology, Writing – review & editing

    Affiliations NAMASTE Center of Excellence, Ljubljana, Slovenia, Institute of Microbiology and Parasitology, Veterinary Faculty, University of Ljubljana, Ljubljana, Slovenia

  • Majda Golob,

    Roles Investigation, Methodology, Writing – review & editing

    Affiliation Institute of Microbiology and Parasitology, Veterinary Faculty, University of Ljubljana, Ljubljana, Slovenia

  • Polona Umek,

    Roles Investigation

    Affiliations Department of Condensed Matter Physics, Jožef Stefan Institute, Ljubljana, Slovenia, NAMASTE Center of Excellence, Ljubljana, Slovenia

  • Zoran Arsov,

    Roles Supervision

    Affiliations Department of Condensed Matter Physics, Jožef Stefan Institute, Ljubljana, Slovenia, NAMASTE Center of Excellence, Ljubljana, Slovenia

  • Goran Dražić,

    Roles Investigation

    Affiliation Department of Materials Chemistry, National Institute of Chemistry, Ljubljana, Slovenia

  • Štefan Pintarič,

    Roles Investigation, Methodology

    Affiliation Institute of Environmental and Animal Hygiene with Animal Behaviour, Veterinary Faculty, University of Ljubljana, Ljubljana, Slovenia

  • Martin Dobeic,

    Roles Conceptualization, Methodology

    Affiliation Institute of Environmental and Animal Hygiene with Animal Behaviour, Veterinary Faculty, University of Ljubljana, Ljubljana, Slovenia

  • Janez Štrancar

    Roles Funding acquisition, Resources, Supervision, Writing – review & editing

    Affiliations Department of Condensed Matter Physics, Jožef Stefan Institute, Ljubljana, Slovenia, NAMASTE Center of Excellence, Ljubljana, Slovenia

Surface deposited one-dimensional copper-doped TiO2 nanomaterials for prevention of health care acquired infections

  • Tilen Koklic, 
  • Iztok Urbančič, 
  • Irena Zdovc, 
  • Majda Golob, 
  • Polona Umek, 
  • Zoran Arsov, 
  • Goran Dražić, 
  • Štefan Pintarič, 
  • Martin Dobeic, 
  • Janez Štrancar


Bacterial infections acquired in healthcare facilities including hospitals, the so called healthcare acquired or nosocomial infections, are still of great concern worldwide and represent a significant economical burden. One of the major causes of morbidity is infection with Methicillin Resistant Staphylococcus aureus (MRSA), which has been reported to survive on surfaces for several months. Bactericidal activity of copper-TiO2 thin films, which release copper ions and are deposited on glass surfaces and heated to high temperatures, is well known even when illuminated with very weak UVA light of about 10 μW/cm2. Lately, there is an increased intrerest for one-dimensional TiO2 nanomaterials, due to their unique properties, low cost, and high thermal and photochemical stability. Here we show that copper doped TiO2 nanotubes produce about five times more ·OH radicals as compared to undoped TiO2 nanotubes and that effective surface disinfection, determined by a modified ISO 22196:2011 test, can be achieved even at low intensity UVA light of 30 μW/cm2. The nanotubes can be deposited on a preformed surface at room temperature, resulting in a stable deposition resistant to multiple washings. Up to 103 microorganisms per cm2 can be inactivated in 24 hours, including resistant strains such as Methicillin-resistant Staphylococcus aureus (MRSA) and Extended-spectrum beta-lactamase Escherichia coli (E. coli ESBL). This disinfection method could provide a valuable alternative to the current surface disinfection methods.


Bacterial infections acquired in healthcare facilities including hospitals, the so called healthcare acquired or nosocomial infections (HAI), are still of great concern worldwide and represent a significant economical burden [1,2]. According to the World Health Organization antimicrobial resistance became an increasingly serious threat to global public health. Namely, many microbial species developed resistance to most newly discovered antibiotic, sometimes even before the drugs were introduced to the market [3,4]. Since the resistance occurs naturally over time, usually through genetic changes, it is inherently associated with the persistence of the bacterial colonization on the surfaces of the buildings, equipment, implants or tools. With its long time scale of many months [5,6], even up to a year [7], it can be thought as a possible long-term source of contamination and recurrent infections as it has been shown in case of medical implants [8]. To protect surfaces and avoid use of antibiotics at the same time, several approaches have been proposed. Silver or copper based antimicrobial surfaces were shown to be effective against different microorganisms, but their widespread usability remains questionable due to inherent copper toxicity to living cells [9], development of silver-resistant bacterial strains [10] and the unresolved environmental and health effects of released ions [11,12]. Even in the case of a more traditional disinfection strategies based on hydrogen peroxide H2O2 [13] or superoxide radical ·O2 [14] cleaning, microbial resistance has been observed [15] with several enzymes responsible for that identified [16]. This is not surprising, since the ·O2 radical and the H2O2 can be enzymatically degraded by superoxide dismutases (2·O2 + 2H+ → H2O2 + O2) and catalases/peroxidases (2H2O2 → 2H2O + O2), respectively. On the other hand, no enzyme is known with ability to catalyze the ·OH [17], which can indiscriminately oxidize organic matter, including DNA [18], presenting a good base to prevent development of antimicrobial resistance. Interestingly, it has been shown that various types of efficient antibiotics, which attack different vital processes in bacteria, increase the production of ·OH hydroxyl radicals inside bacteria [1921]. This suggests that antibacterial effect originates in oxidation caused by the ·OH radical. Taking into account the ability of various types of nanoparticles to produce ·OH radical and the possibility to deposit nanoparticles onto different surfaces, this would undoubtedly present a valuable means for surface antimicrobial protection.

Effectiveness of ·OH generation by TiO2 irradiated with metal halide lamp was demonstrated by Matsunaga et al. already in 1985, when Escherichia coli were completely sterilized [22]. Since then antibacterial effect of photo-excited TiO2 was shown against a wide range of bacteria, fungi, algae, protozoa, viruses, and even bacterial endospores, fungal spores, and protozoan cysts [23]. Based on the knowledge about photocatalytic mechanism and related photochemistry of TiO2 [2427,2731] (Figure A in S1 File) antibacterial action also depends on ·OH radicals, produced on the surface of photo-excited TiO2 with the energy of the light consistent with the TiO2’s bandgap (Figure A in S1 File, reaction ①). Although promising, photocatalytic disinfection of TiO2–based surfaces is not yet widely used. A recent review of commercially available antimicrobial nano-coatings in Europe showed that only one out of 23 antimicrobial coatings was based on the TiO2 [32]. With an average microbial density of several hundred per cm2 in common hospital surfaces [33] to several thousand per cm2 in drawers of frost-free home fridges (as conducted by Microban Europe (Cannock, Staffordshire) and European commission’s recommendation for “clean” food preparation and storage surfaces of less than 10 microbes per cm2, targeted disinfection efficiency is the inactivation of at least 103 microbes/cm2. Indeed, this was achieved recently by Dunlop et al. [34] but at an activation with a rather high intensity UVA light of 30 W/m2. In another study, efficient suppression of growth of Listeria monocytogenes, which can cause dangerous foodborne illness with high mortality rate [35,36], could not be reached even at very high light intensities of up to 90 W/m [37]. We hypothesize that the main reason for such a failure is the same exceptionally high reactivity of the ·OH radical which is able to effectively degrade organic matter. Namely, due to ·OH radical decay by dimolecular reaction in which H2O2 is formed (Figure A in S1 File, reaction ②) [27], concentration of the ·OH radicals could significantly decrease with the distance from the TiO2 surface. A straightforward increase in photo-production of radicals due to higher intensity of light would thus not result in a stronger antimicrobial effect. For this one would needs to transform H2O2 back into ·OH radicals, for example by copper mediated Fenton type reaction [38,39] (Figure A in S1 File, reaction ③). An impact on photocatalytic properties of such a doping of TiO2 with transition metals such as copper has already been shown [40,41]. For example, several research groups made antibacterial coatings based on TiO2 containing copper and tested them at different light intensities [23,24,34,4245]. With an antibacterial effect being not much different from the antibacterial effect achieved in the dark these studies indicate that much of the antibacterial effect is due to leached copper ions [42,43]. It turned out that higher amounts of copper than approximately 1% cannot be successfully incorporated into TiO2 structure, but are deposited as clusters on the TiO2 surface [4648], from which copper can be released into solution. Although it contributes to toxicity of the nanoparticles in absence of irradiation [49] it leads to unacceptable development of copper resistant bacterial strains as well. Another challenge is application of TiO2 materials onto existing surfaces, since manufacturing process often requires high temperatures [34,42,44], thus makes it impossible to protect preformed, temperature sensitive materials. The efficient disinfection strategy should therefore rely exclusively on the incorporation of small amount of copper into TiO2 structure, which could be deposited onto a preformed surface, and activated by very low light intensities.

Recently, interest in one-dimensional TiO2 nanomaterials increased, due to their unique properties, low cost, and high thermal and photochemical stability [50]. Here we show that copper doped TiO2 nanotubes produce about five times more OH radiclas as compared to undoped TiO2 nanotubes and that effective surface disinfection can be achieved even at low intensity UVA light of 30 μW/cm2. The nanotubes can be deposited on a preformed surface at room temperature, resulting in a stable deposition resistant to multiple washings. Up to 103 microorganisms per cm2 can be inactivated in 24 hours, including resistant strains such as Methicillin-resistant Staphylococcus aureus (MRSA) and Extended-spectrum beta-lactamase Escherichia coli (E. coli ESBL).

Materials and methods


The spin trap, 5-(Diethoxyphosphoryl)-5-methyl-1-pyrroline-N-oxide (DEPMPO) (Alexis, Lausen) was used as purchased without further purification and stored at -80°C. The spin-trap stock solutions were always freshly prepared. Ethanol (EtOH) and methanol (MeOH) from Merck AG (Darmstadt, Germany) were used in Lichrosolv® gradient grade quality. Titanium dioxide powder TiO2 (Degussa P25, Germany Degussa Corporation) and rutile TiO2 powder (Aldrich, Titanium(IV) oxide, rutile powder < 5μm) were dispersed in Erlenmeyer flask with KOH to obtain the stock solution of concentration 1 mg/ml. Media and culture materials were obtained from Gibco–Invitrogen Corporation (Carlsbad, California).

Preparation of bacterial inoculum

Antimicrobial properties were tested on non-pathogenic bacterium L. innocua, which is closely related to pathogenic species L. monocytogenes, E. coli, and S. aureus. Suspension of each reference bacterial strain, was supplied by the Institute of Microbiology and Parasitology, Veterinary faculty, University of Ljubljana. Strain was maintained frozen at -70°C in sterile vials containing porous beads which serve as carriers to support microorganisms (Microbank, pro-lab Diagnostics) and kept at -70°C. The inoculum was prepared in liquid medium (Triptose soya broth, TSB, Biolife, Italia) and incubated aerobically for 24 h at 37°C. After incubation the culture contain approximately 109 colony forming units (CFU) per milliliter. Working suspensions with appropriate concentrations were achieved by several 10-fold dilutions. The amount of the initial CFU/mL of the suspension placed in a petri dish was assessed by covering the suspension with approximately 15 mL nutrient agar. After overnight incubation at 37°C colonies were counted to estimate the CFU/mL in the original suspension.

Synthesis and characterization of Cu-doped TiO2 nanotubes

Cu2+-doped TiO2 nanotubes (Cu-TiO2NTs) were prepared in several steps: (i) first sodium titanate nanotubes (Na+-TiNTs) were synthesized from anatase powder (325 mesh, ≥ 99.9%, Aldrich) and 10 M NaOH (aq) (Aldrich) at T = 135°C for 3 days under hydrothermal conditions. Exact synthesis procedure is described previously [51], (ii) in the next step Na+-TiNTs were rinsed with 0.1 M HCl(aq) yielding protonated titanate nanotubes (H+-TiNTs), (iii) then H+-TiNTs were dispersed in 0.5 mM solution of Cu2+(aq) (source of the Cu2+ was CuSO4·5H2O (Riedel de Haen)) and stirred at room temperature for 3 hours. By centrifugation the solid material was separated from the solution containing excess copper, and (iv) finally isolated material was dryed for 10 hours.

The powder X-ray diffraction (XRD) pattern was obtained on a Bruker AXS D4 Endeavor diffractometer using Cu Kα radiation (1.5406 Å; in the 2θ range from 10 to 65°). The elemental compositions of samples were investigated with a field emission scanning electron microscope (FE-SEM (Carl Zeiss, Super 35 LV) equipped with an EDX (energy dispersive X-ray spectrometer) element analysis system. Morphology of the particles in the sample was determined using transmission electron microscope (TEM, Jeol 2100). The specimen for the TEM investigation was prepared by dispersing the sample in MeOH with the help of an ultrasonic bath and depositing a droplet of the dispersion on a lacey carbon-coated copper grid.

Photocatalytic activity of TiO2 nanotubes

The photocatalytic activity of synthesized TiO2 nanomaterials was determined using electron paramagnetic resonance spectroscopy (EPR) with spin trapping, which was optimized for measurement of primary radicals generated in the vicinity of the nanomaterial surface. This was achieved by measuring primary hidroxyl radicals in the presence of 30% ethanol with 5-(Diethoxyphosphoryl)-5-methyl-1-pyrroline-N-oxide spin trap (DEPMPO). EPR spin trapping was applied to measure the generation of reactive oxygen species (ROS) production. On the surface, small pool, proportionate to the size of the sample, was made with silicon paste and was filled with 2 μl of 0,5 M DEPMPO and 18 μl of 30% ethanol and irradiated with 290 nm diode for 5 min. The diode was 1–2 mm above the surface of the sample. The solution with short-lived radicals being trapped in the form of stable DEPMPO spin adducts was then drawn into the quartz capillary of 1 mm diameter, which was put in the 5 mm wide quartz tube and transferred into EPR spectrometer. All EPR measurements were performed on an X-band EPR spectrometer Bruker ELEXYS, Type W3002180. All measurements were recorded at room temperature using 1 Gauss (10−4 T) modulation amplitude, 100 kHz modulation frequency, 20 ms time constant, 15 x 20 seconds sweep time, 20 mW microwave power and 150 G sweep width with center field positioned at 3320 G.

Deposition of Cu-TiO2NTs on surface and testing of the deposition stability

The deposition of Cu-TiO2NTs was made on polystyrene petri dishes (55.4 cm2). Petri dishses were washed before deposition. They were soaked in 20% NaOH solution, rinsed with distilled water, and finally with ethanol vapor. The suspension of the nanotubes with concentration of 1 mg/ml was processed with ultrasonic liquid processor (Sonicator 4000, Misonix) prior to the deposition on the slides. Sonication was performed using 419 MicrotipTM probe, 15 min process time, 10 s pulse-ON time, 10 s pulse-OFF time and maximum amplitude (resulting in 52 W of power). The petri dishes were treated with compressed air 3 times for 3 s. 150 μl of nanoparticle suspension was applied on each petri dish, immediately after compressed air treatment, and smeared evenly. The same number of dishes with nanoparticle deposition and control dishes were prepared for each experiment. On control dishes, only 150 μl of solution was applied. After the deposition, the dishes were left in the oven at 50°C for 2 hours. Then they were rinsed with distilled water and put back in the oven at 50°C for another 2 hours. The amount of deposited material was estimated from EPR signal decrease when soaking the surface with water, alkaline or acidic medium.

Testing antimicrobial activity of Cu-TiO2NTs coated surfaces according to modified ISO 22196:2011

We tested antibacterial activity of Cu-TiO2NTs coated petri dishes (r = 8.4 cm, S = 55.4 cm2) using a slightly modified test according to standard ISO 22196 (Measurement of antibacterial activity on plastics and other non-porous surfaces), a 24-hour inoculation method [32], with different pathogens. We placed 1 mL of each bacterial suspension with different number of bacteria (from 100 to 105 CFU/mL) in a petri dish for 24 hours at 4°C in a refrigerator. Petri dishes were covered with the lid to prevent drying of the suspension during the exposure. The surfaces were illuminated with a LED lamp (characteristics shown in the supplement, Figure F in S1 File) emmiting light at wavelength 360 nm and different light intensities as written in the main text of the manuscript. Next, bacterial suspension in each petri dish was covered with approximately 15 mL of agar at 37°C and incubated for 48 hours at 37°C, finally CFU were counted.

Data reproducibility and statistics

HRTEM images in Fig 1 are representative images of the sample. Data points in Fig 2A are average values of multiple measurements; error bars represent standard errors. Each data point of the: 1) “TiO2NTs” series (Fig 2A, closed grey squares) was measured 2 times (N = 2), 2) “degussa” series (Fig 2A, open circles) was measured 2 to 3 times (N = 2–3), 3) “anatase” series (Fig 2A, open squares) was measured 1 time (N = 1), 4) “Cu-TiO2NTs” series (Fig 2A, closed circles) was measured 3 to 4 times (N = 3–4).

Fig 1. Transmission electron microscopy characterization of Cu-TiO2NTs.

(A) and (B) high resolution transmission electron microscopy (HRTEM); (C) high-angle annular dark-field imaging scanning transmission electron microscopy (HAADF-STEM); (D) annular bright-field scanning transmission electron microscopy (ABF-STEM) and (E) HAADF-STEM of the same region; (F) ABF-STEM and; (G) HAADF-STEM of the same region of the CU doped TiO2 nanotubes with 1.2% of copper with the accompanying line intensity profile, acquired in direction indication by arrow.

Fig 2. Photocatalytic activity of TiO2 nanotubes and TiO2 nanotube coated surface.

A) Hydroxyl radical production at a TiO2 nanotube surface versus illumination wavelength measured at high concentration of the spin trap ethanol (17 M), data points are average values of multiple measurements, error bars represent standard errors; B) Hydroxyl radical production of a TiO2 nanotube coated surface measured at low concentration of spin trap DEPMPO (50mM) illuminated with a light emitting diode with peak wavelength of 320 nm. Height of the bars represent average values of 17 measurements (N = 17); error bars represent standard deviations. Each data point is also shown on the graph as closed squares for “TiO2NTs” series and as closed grey circles for “Cu-TiO2NTs” series.

Height of the bars in Fig 2B represent average values of 17 measurements (N = 17); error bars represent standard deviations. Each data point is also shown on the graph as closed squares for “TiO2NTs” series and as closed grey circles for “Cu-TiO2NTs” series (Fig 2B). Height of bars in Fig 3B and 3C represent average values of 6 measurements for each bar (N = 6); error bars represent standard deviations.

Fig 3. Deposition heterogeneity and stability of copper doped TiO2 nanotubes on a polymer surface.

A) scanning electron microscopy image of TiO2 nanotubes deposited on a surface. B) relative activity of Cu2+-doped TiO2 nanotubes measured after several washing cycles at different pH and normalized to the activity measured before first washing. C) similar relative activity of the Degussa P25 deposition (water—bars with texture with diagonal lines, acid–bars with no texture, base–bars with dotted texture), without abrasion. Height of the bars represent average values of 6 measurements for each bar (N = 6); error bars represent standard deviations.

Height of bars in Fig 4F represents value of regression coefficient a obtained by linear regression f = a*x through all the data points in each frame from A to E: 5 points (N = 5) for “L. inncoua” series, 9 points (N = 9) for “S. aureus” series, 6 points (N = 6) for “MRSA” series, 14 points (N = 14) for “E. coli ESBL” series, and 9 points (N = 9) for “E. coli” series; error bars represent standard error of the regression coefficient.

Fig 4. Antibacterial activity of Cu-TiO2NTs treated petri dishes against different microorganisms.

(A) L. innocua; (B) S. aureus; (C) MRSA; (D) E. coli ESBL; and (E) E. coli. Number of colonies on control surfaces without the antibacterial coating kept in dark for 24 hours at 4°C in a refrigerator are shown as closed grey circles; Number of colonies on Cu-TiO2NTs coated petri dishes illuminated with 300 mW/m2 UVA light for 24 hours at 4°C in a refrigerator are shown as closed red circles; Number of colonies on control surfaces counted directly after inoculation are shown as closed black circles. Vertical arrows in each subframe of the figure represent the uncountable number of colonies (in our case set to 350) Straight lines through the data points represent best fit with only one parameter shown in frame F; (F) reduction of the number of microorganisms with regards to the number of inoculated microorganisms. Height of the bars represents value of regression coefficient a obtained by linear regression f = a*x through all the data points in each frame from A to E: 5 points (N = 5) for “L. inncoua” series, 9 points (N = 9) for “S. aureus” series, 6 points (N = 6) for “MRSA” series, 14 points (N = 14) for “E. coli ESBL” series, and 9 points (N = 9) for “E. coli” series. Error bars represent standard error of the regression coefficient.

Results and discussion

Cu doped TiO2 nanotubes morphology and characteristics

The goal of this study was to produce TiO2 nanoparticles with high photocatalytic activity and small amount of copper ions incorporated into TiO2 lattice, avoiding leaching of the copper ions from the antibacterial surface. In addition, we wanted to develop TiO2 nanoparticles that would adhere better than spherical particles to achieve better stability on a preformed surface. Being aware that transition metal doping of titanate nanostructures results in a change of surface chemistry as well as in catalytic and photocatalytic properties [52], three different methods were considered [47]. Epitaxial growth of metal oxide phases on a surface was immediately excluded since it is more suitable for thin films [53] than for nanoparticle synthesis. On the other hand, ion exchange process using pristine alkali titanate nanostructures (ex situ doping) [52] and growth of sodium titanate nanotubes from already doped TiO2 (in situ doping) [54] produced mixed results: with an in situ doping it was shown that Cu2+ species may intercalate between titanate layers and preserve structure of the nanotubes, whereas in situ method does not produce well-formed nanotubes [47]. Moreover, ex situ doping at high levels of copper (app. 12%) produced nanotubes with Cu2+ species preferentially adsorbed on the surface of the nanotubes in the form of CuO nanoparticles, while doping at low levels of copper (app 0.02%) also produced well-formed nanotubes with more homogeneous distribution of Cu2+ ions. Although the distribution of Cu2+ could not be resolved by electron microscopy, low temperature electron paramagnetic resonance (EPR) method showed that 70% of EPR intensity could be attributed to intercalated Cu2+ ions, suggesting that around 30% of the Cu2+ ions were probably substitutionally doped into the titanate host structure [47].

In order to achieve high amount of incorporated copper ions into the TiO2 host structure, we prepared TiO2 and Cu2+-doped TiO2 nanotubes by calcination in air at 390°C (10 h) of pure hydrogen trititanate nanotubes (HTiNTs) and HTiNTs impregnated with Cu2+ [55,56]. XRD patterns of the TiO2 nanotubes (TiO2NTs) and Cu-doped2+ TiO2 NT (Cu-TiO2NTs) samples (Figure C in S1 File) correspond to anatase (ICDD No. 86–1157). We didn't observe any diffraction peaks belonging to CuO in the XRD pattern of Cu-TiO2NTs probably due to low copper content, 1.2 wt. %, as determined by EDXS analysis. Specific surface area of both samples, measured with BET analysis, is about 120 m2/g. During the transformation from hydrogen titanate to anatase, the nanotube morphology is retained (Figure D in S1 File), but some fragmentation can be observed. Nanotubes in both samples appear to be shorter than in the precursor HTiNTs [55] with the lengths being in the range between 100 and 200 nm and between 20 to 50 nm for the shortest fragments. The average nanotube diameter is about 9 nm, with the full range between 5 and 20 nm. Elemental analysis of the nanotubes confirm the uptake of Cu2+ into Cu-TiO2NTs that look slightly greenish (Figure C in S1 File, bottom) on the contrary to the TiO2NTs that are completely white (Figure C in S1 File, top).

Cu doped TiO2 nanotubes high resolution electron microscopy

To resolve the exact incorporation of copper into the host structure we employed several advanced high resolution electron microscopy techniques. High resolution TEM (HRTEM) images show a crystalline structure of TiO2 nanotubes (Fig 1A and 1B) with no visible amorphous phase at the surface of the nanotubes. By applying a high-angle annular dark-field imaging scanning transmission electron microscopy (HAADF-STEM) we exclude the existence of larger CuO aggregates, since no obvious bright areas in “Z-contrast” imaging was detected (Fig 1C). Using annular bright-field scanning transmission electron microscopy (ABF-STEM), which enables to visualize atomic columns composed of light atoms, we observed thin (0.5 nm) amorphous layer at the surface of some nanotubes(Fig 1D), which is in agreement with XRD data discussed above (Figure C in S1 File), but no brighter contrast in HAADF-STEM (Fig 1E) indicating that no copper is present in this amorphous layer. Intensity distribution along the line indicated by black arrow and presented in the inset of Fig 1G brings us to conclusion that copper atoms indeed incorporate within the host matrix and do not aggregate on the surface of the TiO2 nanotubes.

We also performed electron energy loss spectroscopy (EELS) on the bulk and at the edge of a nanotube (Figure E in S1 File). Since the lower detection limit precludes copper detection in the nanotubes with only 1.2% of copper, it was applied to characterize Ti coordination. At the surface Ti is in lower coordination and possibly in Ti3+ state, whereas in the bulk we can see characteristic octahedrally coordinated Ti4+ EELS spectrum.

Photocatalytic activity of TiO2 nanotubes

We tested the activity of the UV-excited nanotubes by measuring the concentration of photo-generated radicals using electron paramagnetic resonance (EPR) spectroscopy. Although this is a highly sensitive method for detecting paramagnetic species including radicals, some of them, like (and especially) ·OH radicals are so reactive that they never reach high enough concentrations to be detected by EPR. To overcome this, short-lived radicals must be trapped by nitrone compounds forming stable (long-lived) radical adducts, which can then be easily detected and their identity confirmed through their specific hyperfine splitting pattern. Although it has been shown that for some nanoparticles, such as graphene nanosheets, their photocatalytic activity depends on hydroxyl and superoxide radicals as well as holes [57], same is true for TiO2 nanoparticles, however, as shown by Kakuma et al. for anatase TiO2 the rate of ·OH generation is high, as compared with rutile TiO2, whereas the formation rate of ·O2 for rutile is higher than that for anatase [58]. In this work we therefore used the spin trap 5-(dimethoxyphosphoryl)-5′-methyl-1-pyrroline N-oxide (DEPMPO), which is suitable for detecting superoxide radicals as well as hydroxyl radicals [59]. In agreement with the work by Kakuma et al. we identified that main radical produced on our anatase TiO2 nanotubes is the hydroxyl radical, whereas we could not detect the superoxide radical (Figure B in S1 File). By varying the spin trap concentration one can use this method to measure radical concentration on the nanoparticles’ surfaces, where radicals are generated, as well as in the bulk far from the nanoparticles’ surfaces, where radicals oxidize and kill microbes, i.e. where their effect makes a biological impact. In the first case much larger spin trap concentration is needed as compared to the second case. To achieve large enough concentration, we implemented the approach proposed by Adams et al. [60], by which ethanol is added to 30 vol% acting like an efficient and concentrated primary trap, which in addition transforms ·OH radical into a much more stable DEPMPO α-hydroxyethyl radical (CH(CH3)OH) spin adduct instead of DEPMPO-OH [61]. The analysis of the EPR spectra intensities reveals that the amount of ·OH radicals generated on the surface of the Cu2+-doped TiO2 nanotubes (Cu-TiO2NTs) is comparable to the amount generated by undoped TiO2 nanotubes (TiO2NTs) and almost as high as Degussa P25, commercially available spherical TiO2 nanoparticles (Fig 2A). The photocatalytic activity of the original material, from which the TiO2 nanotubes were synthesized, is, as expected, much lower (Fig 2A, open squares).

Photocatalytic activity of a TiO2 nanotube coated surface

Although TiO2 and Cu-doped TiO2 nanoparticles generated similar amount of radicals (Fig 3A), the amount of radicals released from Cu-TiO2NTs far into the solution was approximately 5-times greater than that released from undoped TiO2NTs (Fig 3B). Since low spin trap concentration mimics rare targets like bacteria, which have not overcrowded surface yet, a copper-doped TiO2 nanomaterial provide much more efficient way for the photocatalytic surface disinfection. The presence of the copper atoms, well incorporated into the TiO2 matrix to prevent their release, transform H2O2, a product of the dimolecular reaction [27], back into more reactive ·OH radicals [38,39]. Although these results have been conducted with TiO2 nanotubes deposited on frequently used polystyrene surface via simple droplet deposition, washing and drying, the conclusions can be generalized to different surfaces. Nevertheless, despite the ability to adsorb nanoparticles, there is no other particular constraint on the protected surface.

Deposition stability of Cu2+-doped TiO2 nanotubes on a polymer surface

Once proven that copper-doped TiO2 nanotubes are photochemically active, the deposition heterogeneity and stability were tested to identify the conditions of potential applications. Scanning electron microscopy revealed that Cu-TiO2NTs are fairly uniformly distributed on a polymer surface (Fig 3A). In addition, measurements of the photo-generated ·OH radical concentration after several consequent washings of the Cu-TiO2NTs deposited on a surface and illuminated with UVA light revealed a very stable and chemically-resistant deposition (Fig 3B). On the contrary, deposition of spherical nanoparticles Degussa P25 was found to be less stable (Fig 3C), which can be associated to different morphology of the nanoparticles with the tubes having larger adsorbing surface than the spheres.

Antibacterial activity of Cu-TiO2NTs

Next, we tested antibacterial activity of Cu-TiO2NTs deposited on a polystyrene petri dish (r = 8 cm, S = 50cm2) using a slightly modified test ISO 22196, a 24-hour inoculation method [32], with different bacteria: L. innocua, E. coli, E. coli ESBL and S. aureus including MRSA. L. innocua has been chosen due to close relativity to L. monocytogenes, which has the highest mortality rate among all known foodborne pathogens and its ability to grew at very low temperatures, even at -1.5°C [62], common to food-storage rooms and fridges. Since L. innnocua is an example of Gram-positive bacteria, E. coli has been added to our selection as the very common Gram-negative bacteria. S. aureus has been included to the test as a very frequent strain that can cause many infectious with severe complications. In addition, two antibiotic-resistant bacterial strains MRSA and E. coli ESBL have been selected to check the efficiency against the bacteria that are currently among the biggest challenges in clinical medicine and maintenance of clean hospital infrastructure. Starting contamination concentration range between 10 and 10000 has been decided based on a typical number of bacteria per gram of food or cm2 of surface, which has then been renormalized to the surface of our petri dish. The petri dishes innoculated with the predefined number (as defined above) of the previously selected bacteria have been exposed and continuously illuminated with 300 mW/m2 at the same time for 24 hours at 4°C. Then they were covered with agar and incubated at 37°C for additional 3 days. The colony forming units (CFU) of microorganisms have been counted on petri dishes without the coating (Fig 4, grey circles) and on petri dishes with the Cu-TiO2NTs coating (Fig 4, red circles). To control the bacterial number in the inoculum, the CFU have been counted without the 24 hour UV exposure (Fig 4, black circles). The protection appeared to be very efficient for the majority of the bacterial strains, L. Innocua (Fig 4A), S. aureus (Fig 4B), MRSA (Fig 4C), and E. coli (Fig 4E) with the reduction in the number of inoculated microorganisms of about 103 (Fig 4F). The lowest, but still good result was detected with E. coli ESBL (Fig 4D), where only about 100 microorganisms per selected petri dish surface could be completely inactivated in 24 hours. Additional controls as well as results after exposures to even smaller light intensities are shown in the supplement (Figure H in S1 File). Taking into account the common number of bacteria on the surfaces and that the doubling time of Listeria is more than a day at 4°C [63] (and much longer for other bacteria) such an antibacterial coating would definitively be capable of preventing cross contamination of foods or people getting in contact with different infrastructure parts. The data also show that neither illumination with UVA light of 200 mW/m2 nor coating of TiO2 nanotubes alone could effectivelly suppress the bacterial growth in the targetted range. Instead, one needs a combination of the tested nanomaterial-based coating and illumination of at least 50 mW/m2 of UVA light (Figure H in S1 File).

Visualization and characterization of antimicrobial Cu-TiO2NTs coated surfaces with FMS

To prove the relation between the disinfection efficiency and the contact/proximity between material and bacteria (because of high reactivity of ·OH radical), we tried to co-localize nanotubes and bacteria on the nanotube coated surfaces. To assess the later, we conducted microscopic visual inspection of inoculated surface (by L. innocua only, due to security reasons) that has been previously protected by deposition of tested nanomaterial. The whole sample (with nanotubes and bacteria on) has been stained by rhodamine B isothiocyanate (RITC), which strongly binds to proteins on the surface of bacteria and which at the same time enables identification of TiO2 nanotubes by their modulation of the RITC emission spectrum. Namely, fluorescence properties of rhodamine B are known to be strongly affected by TiO2 via self-photosensitized oxidative transformation [64], which accelerates its bleaching rate and induces a blue spectral shift [65]. In contrast, a red shift was expected when rhodamine molecules form oligomers due to re-absorption and re-emission of fluorescence light [66]—a phenomenon, which would be anticipated in the aggregates of dried probe on PET surface. The chosen dye therefore provides a unique opportunity to discriminate the native polymer surface, the TiO2 nanotubes and bacteria on the same spectrally-contrasted image (Fig 5), acquired by the spectrally-sensitive bleaching-corrected fluorescence microspectroscopy [67,68]. As anticipated, RITC fluorescence on the Cu-TiO2NTs coated surface showed remarkably lower fluorescence emission peak position wavelengths (Fig 5B1) and higher bleaching rates (Fig 5B2) compared to the RITC fluorescence on uncoated surfaces (Fig 5A). In the case when nanomaterial is spread non-uniformly, spectral shift can be used to localize nanomaterial more accurately than by using intensity image alone (Figure M in S1 File, frame B). Note, that bleaching rates (b) span very large range (Fig 5B2) and nicely anti-correlates with the wavelength of the emission maximum (Fig 5B1, λMAX). Individual L. innocua cells were clearly identified on an uncoated surface by higher fluorescence intensity, very low bleaching rates as well as the blue-shifted spectral peak position (Fig 5C1). Thus, bacteria can be identified and counted also throughout the b- λMAX correlation graph (Figure M in S1 File, frame 5 C, red circle on the rightmost graph) as they are always located below the main population line that represent either uncoated polymer surface (at close-to-zero bleaching rate, black ellipsoid) or the TiO2 covered surface (at higher bleaching rates, pink elipsoid).

Fig 5. Characterization of Cu-TiO2NTs coated surfaces inoculated with L. innocua using bleaching-corrected fluorescence microspectroscopy.

All samples were labeled with rhodamine B isothiocyanate (RITC). Column 1: wavelength of the fluorescence emission peak; and Column 2: bleaching rate images are shown for A) control—uncoated polymer surface, B) Cu-TiO2NTs coated surface, C) uncoated surface inoculated with L. innocua, and D) Cu-TiO2NTs coated surface inoculated with L. innocua. The spectrally contrasted images are color coded based on the local values of the associated fluorescence parameter (values for RITC spectral peak position (λMAX) and bleaching rate (b), respectively). Lengths of the scale bars correspond to 10 μm on the sample. The white arrows mark individual bacteria that were identified by the spectral analysis.

After innoculation with bacteria the TiO2-protected polymer surface FMS enables us to localize the bacteria much more reliably than with common fluorescence microscopy, where bacteria and nanoparticles’ aggregates look almost the same (Figure M in S1 File, frame 5 D, leftmost image). Both the wavelength-contrasted as well as the bleaching-rate-contrasted image clearly reveal that bacteria locate more probable on the part of surface without the coating (Fig 5D2, white arrows). Even though microscopy does not provide reliable statistics, a simple visual inspection supported the previously reported results that the coating significantly reduces the number of bacteria. Moreover, no clusters were detected with only few individual bacteria remaining on the areas with sparser coating.

High-resolution visualization of antimicrobial Cu-TiO2NTs coated surfaces with SEM

In addition to fluorescence microscopy, the Cu-TiO2NTs coated surfaces inoculated with L. innocua were inspected also at higher spatial resolution by scanning electron microscopy (SEM), which enables us to discriminate the nanotubes and bacteria based on the shape of objects. The micrographs confirmed that in agreement with fluorescence data shown above, individual bacteria were found mainly in those micro regions without or with much less of the nanomaterial coating. In contrast with the samples without the coating (Fig 6A and 6B), no clusters of organisms were observed on the Cu-TiO2NTs coated surfaces on any of the images, which further indicates the hostility of the coated surface to the microbes.

Fig 6. Scanning electron micrographs of Cu-TiO2NTs coated surfaces inoculated with L. innocua.

A) uncoated surface; B) uncoated surface at higher magnification; C) Cu-TiO2NTs coated surface; D) Cu-TiO2NTs coated surface at higher magnification; bacteria are indicated by white arrows.


The results presented here show that the TiO2 nanotube coated surfaces exhibit high photocatalytic activity when continuously illuminated with low intensity UVA light, efficiently disinfecting the surface against different and also pathogenic bacterial strains. Better understanding of the hydroxyl radical generation and its release from the surface as well as the incorporation of the copper atoms within the TIO2 matrix enabled us to minimize the rapid radical decay into hydrogen peroxide and transform the later back into hydroxyl radical. By this we were able to employ several-folds lower UVA light intensity to achieve the relevant inactivation of bacteria, allowing the application of inexpensive LED light sources. At the same time, maintaining the tube morphology helped us to achieve strong adhesion of the nanotubes to a preformed polymer surfaces, yielding a stable coating which can persist normal washing conditions in various media. Based on these results, we believe that promising new disinfection technology can be developed suitable for maintaining the surfaces clean in food storage and processing systems as well as in preventing persistent bacterial population in hospital infrastructure.

Supporting information

S1 File. Supplement to “Surface deposited one-dimensional copper-doped TiO2 nanomaterials for prevention of health care acquired infections”.



Special thanks to Alma Mehle for measuring data presented in Fig 4B and 4C. We also thanks to Maja Lepen for her excellent technical support in bacteriology laboratory.


  1. 1. Pittet D, Tarara D, Wenzel RP. Nosocomial bloodstream infection in critically ill patients. Excess length of stay, extra costs, and attributable mortality. JAMA. 1994;271: 1598–1601. pmid:8182812
  2. 2. Allegranzi B, Bagheri Nejad S, Combescure C, Graafmans W, Attar H, Donaldson L, et al. Burden of endemic health-care-associated infection in developing countries: systematic review and meta-analysis. Lancet Lond Engl. 2011;377: 228–241.
  3. 3. Kupferschmidt K. Resistance fighters. Science. 2016;352: 758–761. pmid:27174968
  4. 4. Perron GG, Inglis RF, Pennings PS, Cobey S. Fighting microbial drug resistance: a primer on the role of evolutionary biology in public health. Evol Appl. 2015;8: 211–222. pmid:25861380
  5. 5. Bhalla A, Pultz NJ, Gries DM, Ray AJ, Eckstein EC, Aron DC, et al. Acquisition of nosocomial pathogens on hands after contact with environmental surfaces near hospitalized patients. Infect Control Hosp Epidemiol. 2004;25: 164–167. pmid:14994944
  6. 6. Kramer A, Schwebke I, Kampf G. How long do nosocomial pathogens persist on inanimate surfaces? A systematic review. BMC Infect Dis. 2006;6: 130. pmid:16914034
  7. 7. Noimark S, Dunnill CW, Parkin IP. Shining light on materials—A self-sterilising revolution. Adv Drug Deliv Rev. 2013;65: 570–580. pmid:22819684
  8. 8. Høiby N, Bjarnsholt T, Givskov M, Molin S, Ciofu O. Antibiotic resistance of bacterial biofilms. Int J Antimicrob Agents. 2010;35: 322–332. pmid:20149602
  9. 9. Yang M, Li J, Chen PR. Transition metal-mediated bioorthogonal protein chemistry in living cells. Chem Soc Rev. 2014;43: 6511–6526. pmid:24867400
  10. 10. Lima de Silva AA, de Carvalho MAR, de Souza SAL, Dias PMT, da Silva Filho RG, de Meirelles Saramago CS, et al. Heavy metal tolerance (Cr, Ag AND Hg) in bacteria isolated from sewage. Braz J Microbiol Publ Braz Soc Microbiol. 2012;43: 1620–1631. pmid:24031994
  11. 11. De Jong WH, Van Der Ven LTM, Sleijffers A, Park MVDZ, Jansen EHJM, Van Loveren H, et al. Systemic and immunotoxicity of silver nanoparticles in an intravenous 28 days repeated dose toxicity study in rats. Biomaterials. 2013;34: 8333–8343. pmid:23886731
  12. 12. Völker C, Boedicker C, Daubenthaler J, Oetken M, Oehlmann J. Comparative Toxicity Assessment of Nanosilver on Three Daphnia Species in Acute, Chronic and Multi-Generation Experiments. PLOS ONE. 2013;8: e75026. pmid:24116021
  13. 13. Cadnum JL, Mana TSC, Jencson A, Thota P, Kundrapu S, Donskey CJ. Effectiveness of a hydrogen peroxide spray for decontamination of soft surfaces in hospitals. Am J Infect Control. 2015;43: 1357–1359. pmid:26315058
  14. 14. Abreu AC, Tavares RR, Borges A, Mergulhão F, Simões M. Current and emergent strategies for disinfection of hospital environments. J Antimicrob Chemother. 2013;68: 2718–2732. pmid:23869049
  15. 15. Jackett PS, Aber VR, Lowrie DB. Virulence and resistance to superoxide, low pH and hydrogen peroxide among strains of Mycobacterium tuberculosis. J Gen Microbiol. 1978;104: 37–45. pmid:24084
  16. 16. Baureder M, Reimann R, Hederstedt L. Contribution of catalase to hydrogen peroxide resistance in Enterococcus faecalis. FEMS Microbiol Lett. 2012;331: 160–164. pmid:22486165
  17. 17. Dwyer DJ, Kohanski MA, Collins JJ. Role of Reactive Oxygen Species in Antibiotic Action and Resistance. Curr Opin Microbiol. 2009;12: 482–489. pmid:19647477
  18. 18. Imlay JA. Pathways of oxidative damage. Annu Rev Microbiol. 2003;57: 395–418. pmid:14527285
  19. 19. Muers M. Radicals unite antibiotics. Nat News. 2007;
  20. 20. Kohanski MA, Dwyer DJ, Hayete B, Lawrence CA, Collins JJ. A Common Mechanism of Cellular Death Induced by Bactericidal Antibiotics. Cell. 2007;130: 797–810. pmid:17803904
  21. 21. Wright GD. On the Road to Bacterial Cell Death. Cell. 2007;130: 781–783. pmid:17803902
  22. 22. Matsunaga T, Tomoda R, Nakajima T, Wake H. Photoelectrochemical sterilization of microbial cells by semiconductor powders. FEMS Microbiol Lett. 1985;29: 211–214.
  23. 23. Foster HA, Ditta IB, Varghese S, Steele A. Photocatalytic disinfection using titanium dioxide: spectrum and mechanism of antimicrobial activity. Appl Microbiol Biotechnol. 2011;90: 1847–1868. pmid:21523480
  24. 24. Hashimoto K, Irie H, Fujishima A. TiO2 Photocatalysis: A Historical Overview and Future Prospects. Jpn J Appl Phys. 2005;44: 8269–8285.
  25. 25. Emeline AV, Ryabchuk VK, Serpone N. Dogmas and Misconceptions in Heterogeneous Photocatalysis. Some Enlightened Reflections. J Phys Chem B. 2005;109: 18515–18521. pmid:16853384
  26. 26. Herrmann J-M. Fundamentals and misconceptions in photocatalysis. J Photochem Photobiol Chem. 2010;216: 85–93.
  27. 27. Zhang J, Nosaka Y. Mechanism of the OH Radical Generation in Photocatalysis with TiO2 of Different Crystalline Types. J Phys Chem C. 2014;118: 10824–10832.
  28. 28. Yi J, Bahrini C, Schoemaecker C, Fittschen C, Choi W. Photocatalytic Decomposition of H2O2 on Different TiO2 Surfaces Along with the Concurrent Generation of HO2 Radicals Monitored Using Cavity Ring Down Spectroscopy. J Phys Chem C. 2012;116: 10090–10097.
  29. 29. Kakuma Y, Nosaka AY, Nosaka Y. Difference in TiO2 photocatalytic mechanism between rutile and anatase studied by the detection of active oxygen and surface species in water. Phys Chem Chem Phys. 2015;17: 18691–18698. pmid:26120611
  30. 30. Buchalska M, Kobielusz M, Matuszek A, Pacia M, Wojtyła S, Macyk W. On Oxygen Activation at Rutile- and Anatase-TiO2. ACS Catal. 2015;5: 7424–7431.
  31. 31. Zhang J, Nosaka Y. Quantitative Detection of OH Radicals for Investigating the Reaction Mechanism of Various Visible-Light TiO2 Photocatalysts in Aqueous Suspension. J Phys Chem C. 2013;117: 1383–1391.
  32. 32. Molling JW, Seezink JW, Teunissen BE, Muijrers-Chen I, Borm PJ. Comparative performance of a panel of commercially available antimicrobial nanocoatings in Europe. Nanotechnol Sci Appl. 2014;7: 97–104. pmid:25404853
  33. 33. Neely AN, Maley MP. Survival of Enterococci and Staphylococci on Hospital Fabrics and Plastic. J Clin Microbiol. 2000;38: 724–726. pmid:10655374
  34. 34. Dunlop PSM, Sheeran CP, Byrne JA, McMahon MAS, Boyle MA, McGuigan KG. Inactivation of clinically relevant pathogens by photocatalytic coatings. J Photochem Photobiol Chem. 2010;216: 303–310.
  35. 35. Garrido V, García-Jalón I, Vitas AI. Temperature distribution in Spanish domestic refrigerators and its effect on Listeria monocytogenes growth in sliced ready-to-eat ham. Food Control. 2010;21: 896–901.
  36. 36. Røssvoll E, Rønning HT, Granum PE, Møretrø T, Hjerpekjøn MR, Langsrud S. Toxin production and growth of pathogens subjected to temperature fluctuations simulating consumer handling of cold cuts. Int J Food Microbiol. 2014;185: 82–92. pmid:24935689
  37. 37. Rodrigues D, Teixeira P, Tavares CJ, Azeredo J. Food contact surfaces coated with nitrogen-doped titanium dioxide: effect on Listeria monocytogenes survival under different light sources. Appl Surf Sci. 2013;270: 1–5.
  38. 38. Litter MI. Heterogeneous photocatalysis: Transition metal ions in photocatalytic systems. Appl Catal B Environ. 1999;23: 89–114.
  39. 39. Cieśla P, Kocot P, Mytych P, Stasicka Z. Homogeneous photocatalysis by transition metal complexes in the environment. J Mol Catal Chem. 2004;224: 17–33.
  40. 40. You M, Kim TG, Sung Y-M. Synthesis of Cu-Doped TiO2 Nanorods with Various Aspect Ratios and Dopant Concentrations. Cryst Growth Des. 2010;10: 983–987.
  41. 41. Xin B, Wang P, Ding D, Liu J, Ren Z, Fu H. Effect of surface species on Cu-TiO2 photocatalytic activity. Appl Surf Sci. 2008;254: 2569–2574.
  42. 42. Sunada K, Watanabe T, Hashimoto K. Bactericidal Activity of Copper-Deposited TiO2 Thin Film under Weak UV Light Illumination. Environ Sci Technol. 2003;37: 4785–4789. pmid:14594392
  43. 43. Sato T, Taya M. Copper-aided photosterilization of microbial cells on TiO2 film under irradiation from a white light fluorescent lamp. Biochem Eng J. 2006;30: 199–204.
  44. 44. Foster HA, Sheel DW, Sheel P, Evans P, Varghese S, Rutschke N, et al. Antimicrobial activity of titania/silver and titania/copper films prepared by CVD. J Photochem Photobiol Chem. 2010;216: 283–289.
  45. 45. Ditta IB, Steele A, Liptrot C, Tobin J, Tyler H, Yates HM, et al. Photocatalytic antimicrobial activity of thin surface films of TiO(2), CuO and TiO (2)/CuO dual layers on Escherichia coli and bacteriophage T4. Appl Microbiol Biotechnol. 2008;79: 127–133. pmid:18317747
  46. 46. Lock N, Jensen EML, Mi J, Mamakhel A, Norén K, Qingbo M, et al. Copper doped TiO2 nanoparticles characterized by X-ray absorption spectroscopy, total scattering, and powder diffraction–a benchmark structure–property study. Dalton Trans. 2013;42: 9555–9564. pmid:23673489
  47. 47. Umek P, Pregelj M, Gloter A, Cevc P, Jagličić Z, Čeh M, et al. Coordination of Intercalated Cu2+ Sites in Copper Doped Sodium Titanate Nanotubes and Nanoribbons. J Phys Chem C. 2008;112: 15311–15319.
  48. 48. Qiu X, Miyauchi M, Sunada K, Minoshima M, Liu M, Lu Y, et al. Hybrid CuxO/TiO2 Nanocomposites As Risk-Reduction Materials in Indoor Environments. ACS Nano. 2012;6: 1609–1618. pmid:22208891
  49. 49. Wu B, Huang R, Sahu M, Feng X, Biswas P, Tang YJ. Bacterial responses to Cu-doped TiO(2) nanoparticles. Sci Total Environ. 2010;408: 1755–1758. pmid:19931887
  50. 50. Selmani A, Špadina M, Plodinec M, Delač Marion I, Willinger MG, Lützenkirchen J, et al. An Experimental and Theoretical Approach to Understanding the Surface Properties of One-Dimensional TiO2 Nanomaterials. J Phys Chem C. 2015;119: 19729–19742.
  51. 51. Umek P, Korošec RC, Jančar B, Dominko R, Arčon D. The influence of the reaction temperature on the morphology of sodium titanate 1D nanostructures and their thermal stability. J Nanosci Nanotechnol. 2007;7: 3502–8. pmid:18330164
  52. 52. Nian J-N, Chen S-A, Tsai C-C, Teng H. Structural feature and catalytic performance of Cu species distributed over TiO2 nanotubes. J Phys Chem B. 2006;110: 25817–25824. pmid:17181226
  53. 53. Diebold U. The surface science of titanium dioxide. Surf Sci Rep. 2003;48: 53–229.
  54. 54. Huang C, Liu X, Kong L, Lan W, Su Q, Wang Y. The structural and magnetic properties of Co-doped titanate nanotubes synthesized under hydrothermal conditions. Appl Phys A. 2007;87: 781–786.
  55. 55. Sluban M, Cojocaru B, Parvulescu VI, Iskra J, Cerc Korošec R, Umek P. Protonated titanate nanotubes as solid acid catalyst for aldol condensation. J Catal. 2017;346: 161–169.
  56. 56. Umek P, Korosec RC, Jancar B, Dominko R, Arcon D. The influence of the reaction temperature on the morphology of sodium titanate 1D nanostructures and their thermal stability. J Nanosci Nanotechnol. 2007;7: 3502–3508. pmid:18330164
  57. 57. Khare P, Singh A, Verma S, Bhati A, Sonker AK, Tripathi KM, et al. Sunlight-Induced Selective Photocatalytic Degradation of Methylene Blue in Bacterial Culture by Pollutant Soot Derived Nontoxic Graphene Nanosheets. ACS Sustain Chem Eng. 2018;6: 579–589.
  58. 58. Kakuma Y, Nosaka AY, Nosaka Y. Difference in TiO2 photocatalytic mechanism between rutile and anatase studied by the detection of active oxygen and surface species in water. Phys Chem Chem Phys. 2015;17: 18691–18698. pmid:26120611
  59. 59. Frejaville C, Karoui H, Tuccio B, Moigne F le, Culcasi M, Pietri S, et al. 5-Diethoxyphosphoryl-5-methyl-1-pyrroline N-oxide (DEPMPO): a new phosphorylated nitrone for the efficient In Vitro and In Vivo spin trapping of oxygen-centred radicals. J Chem Soc Chem Commun. 1994;0: 1793–1794.
  60. 60. Adams EG, Wardman P. Free Radicals in Biology. III. Pryor WA, editor. New York: Academic Press; 1977. pp. 52–95.
  61. 61. Frejaville C, Karoui H, Tuccio B, Le Moigne F, Culcasi M, Pietri S, et al. 5-(Diethoxyphosphoryl)-5-methyl-1-pyrroline N-oxide: a new efficient phosphorylated nitrone for the in vitro and in vivo spin trapping of oxygen-centered radicals. J Med Chem. 1995;38: 258–65. pmid:7830268
  62. 62. Hudson JA, Mott SJ, Penney N. Growth of Listeria monocytogenes, Aeromonas hydrophila, and Yersinia enterocolitica on Vacuum and Saturated Carbon Dioxide Controlled Atmosphere-Packaged Sliced Roast Beef. J Food Prot. 1994;57: 204–208.
  63. 63. Rosenow EM, Marth EH. Growth of Listeria monocytogenes in Skim, Whole and Chocolate Milk, and in Whipping Cream during Incubation at 4, 8, 13, 21 and 35°C. J Food Prot. 1987;50: 452–463.
  64. 64. Wu T, Liu G, Zhao J, Hidaka H, Serpone N. Photoassisted Degradation of Dye Pollutants. V. Self-Photosensitized Oxidative Transformation of Rhodamine B under Visible Light Irradiation in Aqueous TiO 2 Dispersions. J Phys Chem B. American Chemical Society; 1998;102: 5845–5851.
  65. 65. Watanabe T, Takirawa T, Honda K. Photocatalysis through Excitation of Adsorbates. 1. Highly Efficient N-Deethylation of Rhodamine B Adsorbed to CdS. 1977;81: 1845–1851.
  66. 66. Vogel R, Meredith P, Harvey MD, Rubinsztein-Dunlop H. Absorption and fluorescence spectroscopy of rhodamine 6G in titanium dioxide nanocomposites. Spectrochim Acta A Mol Biomol Spectrosc. 2004;60: 245–9. pmid:14670484
  67. 67. Urbančič I, Arsov Z, Ljubetič A, Biglino D, Strancar J. Bleaching-corrected fluorescence microspectroscopy with nanometer peak position resolution. Opt Express. 2013;21: 25291–306. pmid:24150370
  68. 68. Urbančič I, Ljubetič A, Arsov Z, Strancar J. Coexistence of probe conformations in lipid phases-a polarized fluorescence microspectroscopy study. Biophys J. 2013;105: 919–27. pmid:23972844