Internalization of ferromagnetic nanowires by different living cells
© Prina-Mello et al. 2006
Received: 21 June 2006
Accepted: 05 September 2006
Published: 05 September 2006
Skip to main content
© Prina-Mello et al. 2006
Received: 21 June 2006
Accepted: 05 September 2006
Published: 05 September 2006
The ability of living cells, either adherent or suspended, to internalize nickel nanowires is demonstrated for MC3T3-E1, UMR106-tumour and Marrow-Stromal cells. Nanowires were produced by electrodeposition, 20 μm long and 200 nm in diameter. Cell separation and manipulation was achieved for the three cell types. Applied magnetic field successfully oriented the internalized nanowires but no clear anisotropy is induced on the adherent cells. Nanowires tend to bind to cytoplasm metalloproteins and trigger lysosome reorganization around the nucleus. This work demonstrates the applications of nanowires in adherent and suspended cells for cell separation and manipulation, and further explore into their role in nanobiotechnology.
Ferromagnetic nanoparticles have found widespread uses in modern biology and medicine [1–3]. They are used as contrast agents for magnetic resonance imaging , localized radio-frequency heating  and applying mechanical stress in magnetic tweezers . Applications include functionalized labeling  for separation , drug delivery , imaging and detection . Most current cell labeling techniques use one of two approaches: (1) attaching magnetic nanoparticles to the cell surface or (2) internalizing the nanoparticles by fluid phase endocytosis .
Studies of ferromagnetic nanowires are much less advanced. The advantages over the use of nanowires instead of nanoparticles are related to the favourable geometrical anisotropy, the increased surface to volume ratio and dipolar magnetic properties linked to the nanowire shape. Furthermore by using magnetic nanowires with large permanent magnetic moments it is possible to increase the range and effectiveness of such magnetic interactions to respond to the weak fields at a distance from external magnets.
Techniques are well developed to produce these wires by electrodeposition into porous anodized alumina templates in milligram quantities, and it is possible to tailor their length by changing the deposition time, and their diameter by choosing a suitable template [13, 14, 16]. The wire composition may be uniform or variable along the length of the wire by varying the conditions of electrodeposition. The ability to code information and spatially-varying functionality into the nanowires, as well as their shape anisotropy, means that they have a potentially greater range of useful applications than nanoparticles.
Recently it has been shown by Reich and co-workers [7, 11, 12] that nanowires can be internalized by immortalized fibroblasts, and can be used in biotechnological applications. There, the optimization and yield of magnetic nanowires was carried out as an alternative to magnetic particle separation system and as a cell sorting and positioning system.
The orientation and manipulation of adherent cells by internalized magnetic nanowires has not been extensively exploited . Information in literature is restricted to just one cell type, NIH 3T3 mouse fibroblast cells [7, 11, 12].
Here we investigate a range of cells – undifferentiated, differentiated and tumour cells – and show how they can absorb nickel nanowires in the adherent and suspended states. We investigate the possibility of alignment of these cells in an external magnetic field, with a view towards the alignment of cells for preferential tissue regeneration and bone growth. Finally, we also speculate about the cellular internalization process and activated cytoplasmic mechanism.
The presence of the nanowires made it easy to separate the cells containing a wire from those which did not. The separation experiment was carried out as described above with the MC3T3-E1 and UMR-106 cells. As a result, more than 70 % and 60 % separation purity, defined as the cells captured with nanowires divided by the total number of captured cells, was achieved for MC3T3-E1 cells and UMR cells respectively, which is consistent with the work by Hultgren et. al. . The separated cells were then replated and cultured at physiological condition till confluency, up to 3 days, and then divided for further experimental separation. All the primary cells and cell lineages with internalised magnetic nanowires responded with a total cell survival higher than 95 % (live/death viability/cytotoxicity kit, Molecular Probes, USA) up to 5 days after separation.
A combined staining for lysosomes and mitochondria localized around the nanowire indicates that the internal organelles inside the cytoplasm respond to the nanowire. In parallel to that localized mitochondrial staining also shows lamellipodia extensions due to cell tethering and re-alignment. This could be associated with a nanowire-induced cell stiffening response.
To extend this finding to a larger statistical population, 5 batches, and 100 fields of view were analyzed for each group studied. In total several thousand cells were counted. The quantitative results achieved for the osteosarcoma cells were similar to those reported for the primary MSCs.
The MS cells were time lapse imaged for a total period of 12-hours under phase contrast microscope, which was set so that there was a progressive heating of the culture medium, which led successively to cell detachment from the substrate and subsequent programmed cell death [see Additional file 1]. The video shows floating cells ingesting a nanowire, as well as adherent cells containing a nanowire detaching from the substrate, and eventually undergoing programmed cell death. The dead cells subsequently release part of the cytoplasm and the internalised nanowire.
While it can be seen that there is a clear orientation of the wires in the applied field, the orientation of the cells themselves is barely significant. Several experiments were carried out to investigate the extent of cell alignment versus the anisotropic orientation of the wires.
The viability of the three types of cells is not significantly compromised by the internalization of the nickel nanowires. The cytotoxicity of metallic nickel has been partially discussed in previous studies [7, 17]. There we assessed the cytotoxicity by live/death assay. Cells were culture up to 5 days with a survival rate of 95 %. A critical factor for this survival rate may be the presence of the 3–4 nm oxide layer, inferred from the magnetization measurements and the EDAX analysis. Magnetic properties and quality of the characterized electrodeposited nanowires in this study are comparable with previous studies [14, 16]. Here, we found that the internalization by cells of nanowires with the same length of suspended MC3T3-E1 was promoted by the activation of the plasma membrane receptors associated with the cytoplasm metalloproteins. This was translated into a preferential accumulation of the nanowires close to the cell nucleus membrane, as shown in Fig. 6. The localized activation of lysosomes and mitochondria around the cell nucleus support our results.
In previous works it was highlighted that nickel is an essential structural component of the metalloproteins. Nickel can enter the cell via various routes. Ni2+ ions may enter the cell utilizing the divalent cation receptor  or via the Mg2+ channel, which are both situated in plasma membrane. In other work it was shown that insoluble nickel microparticles can be phagocytised by the cell. The phagocytosis of nickel-containing compounds was enhanced by their crystalline nature, negative surface energy, and appropriate particle size (2–4 μm) . In that study, it was also found that nickel particles fused with lysosomes and were localized around the cell nucleus although speculation were made over the possible mutagenicity of the insoluble nickel content.
Cell separation via nanowires can be done for all these types of cells, which indicates the versatility of the method investigated here for any type of cell manipulation . In this study the multi-lineage approach to the cell separation was implemented for the three types of adherent cells (see Fig. 4, 7 and 8). The wire here drives the anisotropic adhesion of the cells, as shown in Fig. 4. The extension to primary cell then confirmed the effectiveness of the internalization of the nanowires and highlights the difference between adherent and suspended cells (Fig. 8). A future direction is to exploit the functionalization of ferromagnetic nanowires in order to actively control cell-nanowire interaction. This may lead to possible commercial application in biotechnology such as cell purification, cell isolation, cell detection , single cell probing or small volume drug delivery .
The orientation of the wires that have been ingested by the cells is quite clear for suspended cells, where the orientational effect is to be expected, due to the lack of cell adhesion or tethering of the actin filaments. There, a small magnetic field (approx 10 mT) applied to the magnetic nanowires is sufficient to re-orient the floating cells towards the direction of the applied field, since the magnetic energy of the cell containing a nanowire mB ≈ 1.6·10-15 J is much greater than kT ≈ 4·10-21 J. This principle has been used for fibroblast cells (NIH3T3 cells) by Reich and co-workers [7, 11, 12]. There, the optimization and yield of magnetic nanowires was demonstrated as an alternative to magnetic particle separation system and as a cell sorting and positioning system, with a focus on microfluidic applications such parallel plate flow chamber for cell sorting.
On the other hand, the orientation and manipulation of adherent cells by anexternal magnetic field using internalized magnetic nanowires for the alignment of groups of cells may have great potential in tissue differentiation and regeneration . The orientation of different cell lines such as immortalized and primary cells would create a preferential co-culture in the presence of external magnetic stimulus. The main goal here was focused on the orientation of a tumor cell line (UMR 106) and primary cells harvested from adult mouse (marrow stromal cells, MSCs). In both cases the orientation force was induced by the anisotropic alignment of the internalised magnetic nanowires. This was qualitatively investigated for UMR106 (Fig. 7) and quantitatively for MSC, as shown in Fig 9 and 10.
The magnetic torque applied to each cell during the alignment process is approximately mB ≈ 1.6·10-14 Nm. The clear alignment of the nanowires indicates the resistance of the rearrangement of the nanowires is smaller than the cell adhesion force, calculated for human bone marrow stromal cell (HBMSC) (EHBMSC = 3 kPa, cell diam. ≅ 130 μm) .
This is shown in the two histograms reported in Fig. 9. However, in this study we found that there is little correlation between the cell morphology and the orientation of the nanowires, as by comparison of quantitative histograms in figure 9 and figure 10. It is probably either the consequence of the cell-nanowire interaction due to the internalization process or a considerably large mechano-chemical adhesion force exerted by the cells to the surface.
Therefore from the results of this study we can conclude not only that we have successfully achieved the internalization of nanowires on different cell lines (such as MC3T3-E1 osteoblast, Marrow Stromal and UMR106 osteosarcoma cells) but also that the interaction of the nickel nanowires with each cell cytoplasm leads to the internal reorganization of those organelles affected by the nanowires, such as lysosomes and metalloproteins.
Magnetic nanowires open new perspectives for the manipulation, identification and counting of many types of living cells. The viability of different cell types, here shown, is encouraging and opens a new window for the application of ferromagnetic nanowires. Therefore, integration of different magnetic materials inside cells open new prospective in tissue engineering and nanobiotechnology.
Nickel nanowires were grown in alumina membranes (Whatman, UK). The membranes used were 20 mm in diameter and 60 μm thick, with 200 nm parallel-pores spaced by 300 nm. Firstly a gold electrode was deposited on the back of the membrane . Then, nickel was deposited into the pores by electroplating from a NiSO4 bath, at a potential of -0.9 to -1.0 V relative to an Ag, AgCl/KCl reference electrode . The nickel wires were then separated from the membrane by dissolving the alumina membrane in 3 M·l-1 NaOH . The nanowires were then characterized by scanning electron microscopy (Fig. 1), X-ray diffraction (Fig. 2), X-ray fluorescence and vibrating-sample magnetometry (VSM).
In this study three cell lines were used: primary cells from adult rat marrow stromal cells (MSC), MC3T3-E1 osteoblasts cell line and rat osteosarcoma cells (UMR106) (ATCC, USA). Every cell type used in this study was cultured under a different environment and culture medium, in line with the specific cell-culture requirements.
Primary MSCs were cultured and incubated at 37°C, 5 % CO2 and 95 % relative humidity, to confluency with DMEM supplemented with 2 % penicillin/streptomycin (Gibco, UK), 10 % foetal Bovine Serum (FBS; Gibco, UK), 0.5 % l-Glutamine (Gibco, UK), 0.5 % Glutamax (Gibco, UK), and 1 % non-essential amino acids (Gibco, UK).
For the UMR 106 cell line, all samples were cultured and incubated as above with DMEM (30-2002 ATCC, USA) supplemented with 10 % foetal bovine serum, 100 U/ml penicillin and 100 μg/ml streptomycin.
Whereas, MC3T3-E1 were cultured in alpha minimum essential medium (α-MEM: Sigma-Aldrich, UK) containing 10 % foetal bovine serum (FBS; Gibco, UK), 100 U/ml penicillin and 100 μm/ml streptomycin, 2 mM L-glutamine (Gibco, UK) and 0.5 % 100 mM sodium pyruvate (Sigma-Aldrich, UK). The osteoblasts were kept in an incubator at 37°C in a 95 % air 5 % CO2 environment. Subculture was routinely performed at ~80 % confluence, using 0.25 % trypsin.
Nickel nanowires were firstly washed 5 times in deionized water (Ω <= 30 M ohm) and rinsed in different PBS baths. The nanowires were then stabilized for 2 hours into the specifics cell culture medium used for each cell line with a density of 1011 particles/ml and then dispersed by 5 minutes ultrasonic agitation immediately prior to addition. Cell medium-nanowire solution was then added at a final concentration of 106 particles/ml to adhering and suspended cells. Adhering cells were incubated for 30 minutes to promote the internalization of the wires and then incubated overnight. Suspended cells were incubated for 30 minutes and then exposed to magnetic field. After each magnetic exposure, cells on coverslips were subsequently fixed or stained as required for the imaging technique adopted.
Each experiment was repeated several times as part of a larger study to address the extent of nanowires internalization and cell yield.
To characterize the ingestion of nanowires into the cells several imaging and immunofluorescence techniques were used. These were optimized for each cell type to examine the interaction between the cells and the nanowires. In this study all the three cell types were selectively stained for tracking active mitochondria and acidic organelles in live cells to highlight the cell activity during internalization.
The cell staining and preparation was carried out by staining live cells for cell tracking. In this study two cytoskeleton markers were Myto- and Lyso-tracker (Molecular Probes, USA). In brief, after having prepared a 1 mM stock solution of each tracker, a final concentration diluted in the respective growth medium (described above) of 50 nM for Myto-tracker and 50 nM for Lyso-tracker was respectively used to stain samples. Single and double staining on adherent and suspended live cell were carried out for 30 min for Lyso-tracker and 3 min for Myto-tracker; samples were then washed with fresh warm medium and imaging were taken. Subsequent, to live imaging the stained cells were permeabilised and fixed in 4.1 % paraformaldehyde in PBS for 30 min. These concentrations were kept as low as possible in order to reduce possible overloading and artefacts.
Phase contrast, bright-field and time lapse imaging microscopy were carried out with the use of a Zeiss inverted microscope (Zeiss Axiovert 200 M, Germany) connected to a cooled CCD camera (Zeiss Axiocam HRm, Germany).
SEM imaging was carried out on adherent MC3T3-E1 and MSC cells with internalized wires. All cell samples were prepared by fixing each glass coverslip slide with 3 % Glutaraldehyde in 0.1 M Sodium Cacodylate buffer (pH 7.2). The primary fixation was carried out for 1 hour at room temperature. Samples were then washed 6 times for 1 hour with either 0.05 M Phosphate or 0.1 M Cacodylate buffer to remove any un-reacted Glutaraldehyde from the samples before rinse and dehydration was carried out. The samples were then quickly rinsed with 50 % ethanol; dehydrated with 10 %, 30 %, 50 %, 70 %, and 95 % ethanol for 10 min each; and dehydrated with 100 % ethanol twice for 15 min each. The samples were then gold sputter-coated for high resolution imaging.
The ingestion of nanowires into the cells was examined by time lapse contrast microscopy. It was possible to examine the interaction of the cells with the nanowires by programming the Zeiss microscope to acquire an image every 15 minutes for 18 hrs (as reported in the supplemental material video). There, the light was programmed to heat the medium so that both adherent and floating cells could be examined.
The cell separation set-up was made of two Nd2Fe14B permanent magnets of 10 mm diameter and 15 mm length in antiparallel configuration at opposite sides of a 10 ml falcon tube for cell suspension. The surface magnetic field of the magnets of 0.6 T was measured by hall sensor gaussmeter (Hirst, UK). The two magnets fixed on either side of the tube together produced a magnetic field gradient up to 100 T/m.
Cells cultured with nanowires were dissociated with warmed trypsin plus EDTA4Na solution (Sigma-Aldrich, UK) for 5 min. From each full batch half was put into the magnetic separation set-up, and the other half was replated with 3 ml of fresh medium to estimate the amount of cell binding with nanowires pre-separation.
The magnetic separation was carried out for 5 minutes in order to obtain the complete sedimentation of those cells without nanowires. These last, after separation were removed and plated in 3 ml fresh medium in a new Petri dish. After having removed the magnets, the cells with nanowires were dispersed into 3 ml of fresh medium and replated in a new Petri dish.
Complete cell adhesion was achieved in less then 1 h of incubation at physiological conditions for all the batches and then cell counting was carried out in 2–3 rounds to minimize systematic and operator errors. Images were captured using an Olympus BX41 microscope (Japan) with magnifications of 10×, 20×, and 40× connected to a cooled CCD camera (Image II, USA). All images were acquired and stored by using Analysis imaging software (Analysis, Germany).
For the nanowire and cell alignment test, a uniform magnetic field of 100 mT was applied by a cylindrical Halbach permanent magnet made of segments of Nd2Fe14B (Magnetic Solutions, Ireland). The inner and outer radii of the magnet were 106 and 156 mm, respectively. Cells with Ni nanowires were co-cultured overnight before the test. The duration of the magnetic field exposure was chosen to be 1 hr, 24 hrs or 48 hrs inside an incubator at physiological conditions (T = 37°C, CO2 = 5 % and RH = 95 %). Subsequently, images were taken under phase contrast as described above. The degree of alignment of the wires and cell morphology to the direction of the field was conducted by using Scion Image software (Scion Corporation, USA). Both cell and nanowire counting were carried out under blind conditions to reduce systematic errors.
The authors thank L. McMahon, E. Kearney, and Dr. E. Byrne for their technical assistance, and Dr. P. Maguire for her valuable discussions. The authors also thank Prof. P.J. Prendergast, Dr. V. Campbell and Dr. S. Jarvis for the use of their laboratories and facilities.
Science Foundation Ireland for the financial support, under the SFI CINSE and CRANN exploratory projects. Mr. Zhu Diao for the Ussher Fellowship from Trinity College Dublin, Ireland.
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.