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	<ui>1556-276X-7-358</ui>
	<ji>1556-276X</ji>
	<fm>
		<dochead>Nano Express</dochead>
		<bibl>
			<title>
				<p>Shape engineering vs organic modification of inorganic nanoparticles as a tool for enhancing cellular internalization</p>
			</title>
			<aug>
				<au id="A1"><snm>Karaman</snm><mnm>Sen</mnm><fnm>Didem</fnm><insr iid="I1"/><email>dsen@abo.fi</email></au>
				<au id="A2"><snm>Desai</snm><fnm>Diti</fnm><insr iid="I1"/><insr iid="I2"/><email>ddesai@abo.fi</email></au>
				<au id="A3"><snm>Senthilkumar</snm><fnm>Rajendran</fnm><insr iid="I3"/><email>biosen81@gmail.com</email></au>
				<au id="A4"><snm>Johansson</snm><mi>M</mi><fnm>Emma</fnm><insr iid="I4"/><email>emmjo@ifm.liu.se</email></au>
				<au id="A5"><snm>R&#229;tts</snm><fnm>Natalie</fnm><insr iid="I1"/><insr iid="I3"/><insr iid="I5"/><email>nratts@abo.fi</email></au>
				<au id="A6"><snm>Od&#233;n</snm><fnm>Magnus</fnm><insr iid="I4"/><email>magod@ifm.liu.se</email></au>
				<au id="A7"><snm>Eriksson</snm><mi>E</mi><fnm>John</fnm><insr iid="I3"/><email>jeriksso@abo.fi</email></au>
				<au id="A8"><snm>Sahlgren</snm><fnm>Cecilia</fnm><insr iid="I3"/><insr iid="I5"/><email>csahlgre@btk.fi</email></au>
				<au id="A9"><snm>Toivola</snm><mi>M</mi><fnm>Diana</fnm><insr iid="I3"/><insr iid="I6"/><email>dtoivola@abo.fi</email></au>
				<au id="A10" ca="yes"><snm>Rosenholm</snm><mi>M</mi><fnm>Jessica</fnm><insr iid="I1"/><email>jerosenh@abo.fi</email></au>
			</aug>
			<insg>
				<ins id="I1"><p>Centre for Functional Materials, Laboratory of Physical Chemistry, Department of Natural Sciences, &#197;bo Akademi University, Porthansgatan 3-5, Turku, FI-20500, Finland</p></ins>
				<ins id="I2"><p>Pharmacy Department, Faculty of Tech. &amp; Eng, The M.S. University of Baroda, Vadodara, Gujarat -390002, India</p></ins>
				<ins id="I3"><p>Department of Biosciences, Cell biology, &#197;bo Akademi University, Artillerigatan 6A, Turku FI-20520, Finland</p></ins>
				<ins id="I4"><p>Nanostructured Materials Division, Department of Physics, Chemistry and Biology, Link&#246;ping University, Link&#246;ping, SE-581 83, Sweden</p></ins>
				<ins id="I5"><p>Turku Centre for Biotechnology, University of Turku and &#197;bo Akademi University, P.O. Box 123, Turku FI-20521, Finland</p></ins>
				<ins id="I6"><p>Turku Center for Disease Modeling, Kiinamyllynkatu 10, Turku FIN-20520, Finland</p></ins>
			</insg>
			<source>Nanoscale Research Letters</source>
			<issn>1556-276X</issn>
			<pubdate>2012</pubdate>
			<volume>7</volume>
			<issue>1</issue>
			<fpage>358</fpage>
			<url>http://www.nanoscalereslett.com/content/7/1/358</url>
			<xrefbib><pubidlist><pubid idtype="doi">10.1186/1556-276X-7-358</pubid><pubid idtype="pmpid">22747910</pubid></pubidlist></xrefbib>
		</bibl>
		<history><rec><date><day>3</day><month>4</month><year>2012</year></date></rec><acc><date><day>23</day><month>5</month><year>2012</year></date></acc><pub><date><day>1</day><month>7</month><year>2012</year></date></pub></history>
		<cpyrt><year>2012</year><collab>Sen Karaman et al.; licensee Springer.</collab><note>This is an Open Access article distributed under the terms of the Creative Commons Attribution License (
				<url>http://creativecommons.org/licenses/by/2.0</url>), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.</note></cpyrt>
		<kwdg>
			<kwd>mesoporous silica nanoparticles</kwd>
			<kwd>surface functionalization</kwd>
			<kwd>rod-shaped particles</kwd>
			<kwd>surface charge</kwd>
			<kwd>cellular internalization</kwd>
			<kwd>nanomedicine</kwd>
		</kwdg>
		<abs>
			<sec>
				<st>
					<p>Abstract</p>
				</st>
				<p>In nanomedicine, physicochemical properties of the nanocarrier affect the nanoparticle's pharmacokinetics and biodistribution, which are also decisive for the passive targeting and nonspecific cellular uptake of nanoparticles. Size and surface charge are, consequently, two main determining factors in nanomedicine applications. Another important parameter which has received much less attention is the morphology (shape) of the nanocarrier. In order to investigate the morphology effect on the extent of cellular internalization, two similarly sized but differently shaped rod-like and spherical mesoporous silica nanoparticles were synthesized, characterized and functionalized to yield different surface charges. The uptake in two different cancer cell lines was investigated as a function of particle shape, coating (organic modification), surface charge and dose. According to the presented results, particle morphology is a decisive property regardless of both the different surface charges and doses tested, whereby rod-like particles internalized more efficiently in both cell lines. At lower doses whereby the shape-induced advantage is less dominant, charge-induced effects can, however, be used to fine-tune the cellular uptake as a prospective &#8216;secondary&#8217; uptake regulator for tight dose control in nanoparticle-based drug formulations.</p>
			</sec>
		</abs>
	</fm>
	<bdy>
		<sec>
			<st>
				<p>Background</p>
			</st>
			<p>Whereas nanotechnology seeks to engineer and apply the unique properties of materials that emerge when the dimensions enter the nanoscale, nanomedicine attempts to exploit these for the benefit of human health. Nanomaterials in this context are intriguing because they can resemble biological &#8216;nanomachines&#8217; (such as biomacromolecules) as they meet on the same length scale 
				<abbrgrp>
					<abbr bid="B1">1</abbr>
				</abbrgrp> and, thus, can be expected to perform similar tasks or at least possess reminiscent biobehavior. One of the properties exploited in nanomedicine is the ability of nanoparticles to enter cells, whereby they can function as efficient carriers for intracellular drug delivery. The behavior of nanomaterials on the nano-bio interface is largely determined by the physicochemical properties of the nanocarrier, of which size and surface charge have been emphasized as the two most critical ones. Another design parameter that has not received as much attention to date is particle shape 
				<abbrgrp>
					<abbr bid="B2">2</abbr>
				</abbrgrp>. Available results suggest that, as compared to their spherical counterparts, elongated nanoparticles could be more favorable for therapeutic applications based on targeting specificity, biodistribution as well as cellular internalization profiles 
				<abbrgrp>
					<abbr bid="B3">3</abbr>
				</abbrgrp>. On this topic, it has been suggested that the resemblance of rod-like particles with rod-like bacteria could be a reason for the observed advantages in internalization rates in non-phagocytic cells 
				<abbrgrp>
					<abbr bid="B4">4</abbr>
				</abbrgrp>. Particles that, in such a way, mimic properties such as size, shape and flexibility of naturally occurring entities (for instance, circulating cells, e.g., red blood cells) may offer advantages that are typically not observed for standard (polymeric) particles 
				<abbrgrp>
					<abbr bid="B5">5</abbr>
				</abbrgrp>.</p>
			<p>One reason for the general scarcity of the shape-dependency effects on biological performance is the more difficult fabrication of nanoparticles with controlled rod-like morphology due to surface energy minimization during synthesis, leading to spherical shapes 
				<abbrgrp>
					<abbr bid="B6">6</abbr>
				</abbrgrp>. Especially for more novel materials' classes, the first hurdles to overcome include obtaining well-dispersed, monosized particles throughout all processing steps 
				<abbrgrp>
					<abbr bid="B7">7</abbr>
				</abbrgrp>. One promising materials' class in the sense of nanomedicine is mesoporous silica, which can be produced with nanoscale particle diameters and with tunable properties when it comes to both particle size and morphology, meso (pore) structure and size as well as surface chemistry 
				<abbrgrp>
					<abbr bid="B8">8</abbr>
				</abbrgrp>. The controllable characteristics of these materials have boosted research regarding their potential use within the biomedical field during the last decade, especially so for targeted cancer therapy and diagnostics 
				<abbrgrp>
					<abbr bid="B9">9</abbr>
					<abbr bid="B10">10</abbr>
					<abbr bid="B11">11</abbr>
				</abbrgrp>. Mesoporous silica nanoparticles (MSNs) have been successfully loaded with a range of different chemotherapeutics for efficient intracellular delivery and subsequent elimination of the cancer cells. A vast array of sizes and surface modifications have been produced and studied both <it>in vitro</it> and <it>in vivo</it>, while only a few studies have been devoted to the shape effect on MSN biobehavior 
				<abbrgrp>
					<abbr bid="B12">12</abbr>
					<abbr bid="B13">13</abbr>
					<abbr bid="B14">14</abbr>
					<abbr bid="B15">15</abbr>
					<abbr bid="B16">16</abbr>
				</abbrgrp>. To add to the increased understanding of shape-induced effects for MSNs, we have, in this study, synthesized two similarly sized but differently shaped rod-like (NR-MSP) and spherical (S-MSP) fluorescently labeled mesoporous silica nanoparticles in order to investigate the morphology effect on cellular internalization. Additionally, both the rods and spheres were functionalized to yield different surface charges in order to distinguish morphology from surface charge-induced effects and, in the best case scenario, find the dominant parameter. <it>In vitro</it> studies were carried out in two different cancer cell lines, HeLa (cervical carcinoma cells) and Caco-2 (human epithelial colorectal adenocarcinoma cells), to investigate the particle characteristic impact on cells of different origin. According to our results, all of the studied factors (particle shape, surface charge, the nature of the coating as well as the targeted cell populations) are important to be considered when designing new nanocarrier formulations for targeted cancer therapies or other potent drugs that require tight dose control.</p>
		</sec>
		<sec>
			<st>
				<p>Methods</p>
			</st>
			<sec>
				<st>
					<p>Particle preparation and characterization</p>
				</st>
				<p>The synthesis and functionalization of spherical and rod-like MSNs have been summarized below in Figures 
					<figr fid="F1">1</figr> and 
					<figr fid="F2">2</figr>, respectively.</p>
				<fig id="F1"><title><p>Figure 1 </p></title><caption><p>Brief summary of the formation of spherical and rod-like mesoporous silica nanoparticles (denoted MSP)</p></caption><text>
   <p>
      <b>Brief summary of the formation of spherical and rod-like mesoporous silica nanoparticles (denoted MSP).</b>
   </p>
</text><graphic file="1556-276X-7-358-1"/></fig>
				<fig id="F2"><title><p>Figure 2 </p></title><caption><p>The applied surface functionalization procedures for spherical and rod-shaped mesoporous silica nanoparticles</p></caption><text>
   <p>
      <b>The applied surface functionalization procedures for spherical and rod-shaped mesoporous silica nanoparticles.</b>
   </p>
</text><graphic file="1556-276X-7-358-2"/></fig>
			</sec>
			<sec>
				<st>
					<p>Spherical mesoporous silica particles</p>
				</st>
				<p>S-MSP<sub>1</sub> was synthesized according to the protocol described in reference 
					<abbrgrp>
						<abbr bid="B17">17</abbr>
					</abbrgrp>, with slight modifications and details given in Additional file 
					<supplr sid="S1">1</supplr>. In order not to alter the surface charge of the particles, fluorescein isothiocyanate (FITC)-modified aminopropyltriethoxysilane silane (APTES) was mixed with the silica source before adding to the reaction solution to provide co-condensed functionalization of FITC within the silica framework. The modification of APTES was carried out by pre-reacting FITC with APTES in 2&#8201;mL acetone with a molar ratio of 1:3 and stirring for 2&#8201;h under inert atmosphere. The molar ratio between APTES and tetraethyl orthosilicate (TEOS) was kept as 1:100. The thus-preserved negative surface charge was subsequently utilized for further electrostatic adsorption of branched 25&#8201;k poly(ethylene imine) (PEI) to the surfactant-extracted particles (S-MSP<sub>1</sub>-PEI adsorbed). The functionalization of S-MSP<sub>1</sub> was carried out by overnight adsorption (Figure&#8201;
					<figr fid="F2">2</figr>) in 4-(2-hydroxyethyl)-1-piperazineethanesulfonic acid (HEPES) buffer at neutral pH, after which, the particles were collected by centrifugation and washed excessively with deionized water to remove excess PEI.</p>
				<suppl id="S1">
					<title>
						<p>Additional file 1</p>
					</title>
					<text>
						<p>
							<b> Supplementary methods.</b>
						</p>
					</text>
					<file name="1556-276X-7-358-S1.docx">
   <p>Click here for file</p>
</file>
				</suppl>
				<p>S-MSP<sub>2</sub> was synthesized according to our previously published protocols 
					<abbrgrp>
						<abbr bid="B18">18</abbr>
					</abbrgrp>, with FITC added in the synthesis step to create inherently fluorescent particles. In this case, no pre-reaction between the aminosilane and FITC was needed as the amount of aminosilane used in the synthesis was considerable (10&#8201;mol%), and the reaction conditions are favorable also for FITC conjugation. As the surface charge of the MSPs prepared according to this protocol is neutral to slightly positive, electrostatic adsorption of PEI is not possible. Thus, these particles were PEI-functionalized by surface growing of PEI 
					<abbrgrp>
						<abbr bid="B19">19</abbr>
						<abbr bid="B20">20</abbr>
						<abbr bid="B21">21</abbr>
					</abbrgrp> to yield sample S-MSP<sub>2</sub>-PEI grafted (Figure&#8201;
					<figr fid="F2">2</figr>).</p>
			</sec>
			<sec>
				<st>
					<p>Rod-like mesoporous silica particles</p>
				</st>
				<p>NR-MSPs were synthesized according to reference 
					<abbrgrp>
						<abbr bid="B22">22</abbr>
					</abbrgrp>, with TEOS as silica source and block-co-polymer P123 (EO<sub>20</sub>PO<sub>70</sub>EO<sub>20</sub>) as pore-structuring agent in the presence of NH<sub>4</sub>F and heptane. Contrary to the S-MSP syntheses, the nanorod (NR) synthesis is performed under acidic conditions, where the particle length and width can be tuned with the aid of HCl concentration. The synthesis solution consisted of a molar ratio of 1 P123/1.8 NH<sub>4</sub>F/280 Heptane/60 TEOS/356 HCl/10335 H<sub>2</sub>O. The synthesis was kept under vigorous stirring for 4&#8201;min and subsequently, under static conditions for 1&#8201;h. Then, the solution was transferred to a closed Teflon flask for hydrothermal treatment at 100&#176;C for 24&#8201;h. The resulting product was filtered and washed with distilled water. Finally, the material was calcined at 550&#176;C for 5&#8201;h in order to remove the structure-directing agent (SDA) P123.</p>
				<p>The produced nanorods were subsequently fluorescently labeled post-synthesis using the same pre-reaction solution as was added already in the synthesis step for S-MSP<sub>1</sub>. Thus, the negative surface charge of the NR-MSPs could also be preserved, and as a comparison to both S-MSPs, the NR-MSPs were PEI-functionalized both by surface grafting (NR-MSP-PEI graf.) and electrostatic adsorption (NR-MSP-PEI ads.). Furthermore, to investigate the surface charge effect of NR-MSPs, the NR-MSP-PEI graf. samples were further functionalized via either succinylation to yield negatively charged succinic acid groups 
					<abbrgrp>
						<abbr bid="B21">21</abbr>
						<abbr bid="B23">23</abbr>
					</abbrgrp> (NR-MSP-PEI-SUCC) or capping of the primary amines with uncharged acetyl groups 
					<abbrgrp>
						<abbr bid="B24">24</abbr>
					</abbrgrp> (NR-MSP-PEI-ACA). For both functionalization regimes, the PEI-functionalized particles were dispersed in DMF, into which either succinic or acetic anhydride was added in excess. The reaction suspension was agitated overnight. Next day, the particles were separated by centrifugation, washed with absolute ethanol and vacuum dried or directly dispersed into dimethyl sulfoxide (DMSO) at a concentration of 5&#8201;mg/ml for cellular experiments.</p>
			</sec>
			<sec>
				<st>
					<p>Particle characterization methods</p>
				</st>
				<p>Thermogravimetrical analysis (Netzsch TG 209) was used to determine the amount of PEI added at temperature intervals of 170&#176;C to 770&#176;C. Successful modification of PEI and further derivatization with succinic acid or acetyl groups were further confirmed by zeta potential measurements (Malvern ZetaSizer NanoZS, Malvern Instruments Ltd., Worcestershire, UK). Full redispersibility of dried, extracted and surface-functionalized particles was confirmed by redispersion of dry particles in HEPES buffer at pH 7.2 and subsequent dynamic light scattering (DLS) measurements (Malvern ZetaSizer NanoZS). Scanning electron microscopy (SEM; Jeol JSM-6335&#8201;F (JEOL Ltd., Tokyo, Japan) for S-MSPs and Leo 1550 Gemini SEM (Zeiss, Oberkochen, Germany) for NR-MSPs) further confirmed the size, monodispersity, morphology and non-agglomerated state of the particles. The mesoscopic ordering of the nanoparticles was further confirmed by transmission electron microscopy (FEI Tecnai 12 TEM (FEI Co., Hillsboro, OR, USA) operating at 120&#8201;kV with a LaB6 filament and a 2&#8201;k&#8201;&#215;&#8201;2&#8201;k CCD camera) as well as powder XRD using a Kratky compact small-angle system (MBraun, Nottinghampshire, UK). The structural parameters related to the mesoporosity (surface area, pore size and pore volume) were determined by nitrogen sorption measurements (ASAP 2020 (Micromeritics Instrument Corp., Norcross, GA, USA) for NR-MSPs and Autosorb 1 (Quantachrome, Boynton Beach, FL, USA) for S-MSPs). Successful incorporation of fluorescein was determined by fluorescence spectrometry (Perkin Elmer LS 50B, PerkinElmer, Waltham, MA, USA) of particles dispersed in HEPES at a concentration of 0.5&#8201;mg/ml by excitation at 490&#8201;nm and determining the fluorescence intensity at wavelength 520&#8201;nm.</p>
			</sec>
			<sec>
				<st>
					<p>Cell culturing, fluorescence-assisted cell sorting and cytotoxicity</p>
				</st>
				<sec>
					<st>
						<p>Cell lines</p>
					</st>
					<p>HeLa cells and Caco-2 cells obtained from ATCC (Manassas, VA, USA) were maintained in DMEM medium (Sigma, St. Louis, MO, USA) supplemented with 10% fetal calf serum (BioClear, Wiltshire, UK), 2&#8201;mM&#8201;L-glutamin, 100 U/ml penicillin and 100&#8201;&#956;g/ml streptomycin at 37&#176;C in a 5% CO<sub>2</sub>/95% O<sub>2</sub> and 90% RH humidified atmosphere and handled under sterile conditions.</p>
				</sec>
				<sec>
					<st>
						<p>Cellular uptake by fluorescence-assisted cell sorting and confocal fluorescence microscopy</p>
					</st>
					<p>MSPs were suspended in a cell medium at different concentrations (1, 2 and 10&#8201;&#956;g/ml) according to details given in Additional file 
						<supplr sid="S1">1</supplr>. The amount of endocytosed particles inside the cells was analyzed by BD FacsCalibur flow cytometer (FL-I, BD Pharmingen, San Jose, CA, USA). The mean fluorescence intensity (MFI) of the cells at FL-1 channel was measured. The data were analyzed with BD CellQuest Pro&#8482; software for the total amount of MSP uptake by 10,000 cells. GraphPad Prism 5.0 software was used for the statistical analysis of the results. The bar graphs in the figures represent mean values (&#177;SD) from four or more independent experiments.</p>
					<p>For microscopical studies, HeLa cells were seeded on a glass-bottom chamber slide (Lab-Tek&#8482;, Brendale, Australia) and incubated as explained in Additional file 
						<supplr sid="S1">1</supplr>. The cells were viewed with Leica TCS SP5 confocal microscope (Leica Micosystems, Wetzlar, Germany; &#215;63 oil objective, 488&#8201;nm/514&#8201;nm/543&#8201;nm excitation).</p>
				</sec>
				<sec>
					<st>
						<p>Cell viability by WST-1 assay</p>
					</st>
					<p>HeLa cells were transferred to 96-well plates (9,000 cells/well) and allowed to attach and grow. After 24&#8201;h, the medium was removed and replaced with 100&#8201;&#956;l medium containing different concentrations of MSPs (10 and 25&#8201;&#956;g/ml). After incubation for 12&#8201;h, 10&#8201;&#956;l of WST-1 (Roche Applied Science, Upper Bavaria, Germany) reagent was added to the cells, and further incubated for 90&#8201;min; after which, the 96-well plate was analyzed at a 430-nm wavelength in a Varioskan plate reader (Thermo Scientific, Logan UT, USA) to determine cell viability. Here, negative control (NC) is the cell media only without particles, NC DMSO-cell is the cell media with particle vehicle (DMSO), and positive control (PC) is with calyculin A (50&#8201;ng/ml) added to the cell media.</p>
				</sec>
			</sec>
		</sec>
		<sec>
			<st>
				<p>Results</p>
			</st>
			<p>The characteristics of the produced particles in suspension form (0.5&#8201;mg/ml HEPES buffer) have been summarized in Table 
				<tblr tid="T1">1</tblr>. The PEI amount (in weight percent with respect to the whole particle system) as determined from thermogravimetrical analysis was around 10&#8201;wt.% for all PEI-modified particles.</p>
			<table id="T1">
				<title>
					<p>Table 1</p>
				</title>
				<caption>
					<p>
						<b>Characteristics of silica nanoparticle suspensions (0.5&#8201;mg/ml) in HEPES buffer (25&#8201;mM, pH 7.2)</b>
					</p>
				</caption>
				<tgroup align="left" cols="4">
					<colspec align="left" colname="c1" colnum="1" colwidth="1*"/>
					<colspec align="left" colname="c2" colnum="2" colwidth="1*"/>
					<colspec align="left" colname="c3" colnum="3" colwidth="1*"/>
					<colspec align="left" colname="c4" colnum="4" colwidth="1*"/>
					<thead valign="top">
						<row rowsep="1">
							<entry colname="c1">
								<p>
									<b>Sample</b>
								</p>
							</entry>
							<entry colname="c2">
								<p>
									<b>Hydrodynamic Size (nm)</b>
								</p>
							</entry>
							<entry colname="c3">
								<p>
									<b>Zeta potential (mv)</b>
								</p>
							</entry>
							<entry colname="c4">
								<p>
									<b>Fluorescence intensity at</b><b>&#8201;<it>&#955;</it>&#8201;</b>&#8201;<b>=&#8201;520&#8201;nm</b>
								</p>
							</entry>
						</row>
					</thead>
					<tfoot>
						<p>NR-MSP, rod-like mesoporous silica particles; NR-MSP-PEI-ACA, acetic anhydride-modified NR-MSP-PEI graf.; NR-MSP-PEI ads., 25&#8201;k poly(ethylene imine)-adsorbed NR-MSP; NR-MSP-PEI graf., poly(ethylene imine) surface-grown NR-MSP; NR-MSP-PEI-SUCC, succinic anhydride-modified NR-MSP-PEI graf.; S-MSP<sub>1</sub>, negatively charged spherical mesoporos silica nanoparticles; S-MSP<sub>2</sub>, neutrally charged spherical mesoporos silica nanoparticles; S-MSP<sub>1</sub>-PEI ads., 25&#8201;k poly(ethylene imine)-adsorbed S-MSP<sub>1</sub>; S-MSP<sub>2</sub>-PEI graf., poly(ethylene imine) surface-grown S-MSP<sub>2</sub>.</p>
					</tfoot>
					<tbody valign="top">
						<row>
							<entry colname="c1">
								<p>S-MSP<sub>1</sub>
								</p>
							</entry>
							<entry colname="c2">
								<p>687</p>
							</entry>
							<entry colname="c3">
								<p>&#8722;18</p>
							</entry>
							<entry colname="c4">
								<p>567</p>
							</entry>
						</row>
						<row>
							<entry colname="c1">
								<p>S-MSP<sub>2</sub>
								</p>
							</entry>
							<entry colname="c2">
								<p>875</p>
							</entry>
							<entry colname="c3">
								<p>&#8776;0</p>
							</entry>
							<entry colname="c4">
								<p>392</p>
							</entry>
						</row>
						<row>
							<entry colname="c1">
								<p>NR-MSP</p>
							</entry>
							<entry colname="c2">
								<p>470</p>
							</entry>
							<entry colname="c3">
								<p>&#8722;16</p>
							</entry>
							<entry colname="c4">
								<p>626</p>
							</entry>
						</row>
						<row>
							<entry colname="c1">
								<p>S-MSP<sub>1</sub>-PEI ads.</p>
							</entry>
							<entry colname="c2">
								<p>692</p>
							</entry>
							<entry colname="c3">
								<p>22</p>
							</entry>
							<entry colname="c4">
								<p>216</p>
							</entry>
						</row>
						<row>
							<entry colname="c1">
								<p>S-MSP<sub>2</sub>-PEI graf.</p>
							</entry>
							<entry colname="c2">
								<p>569</p>
							</entry>
							<entry colname="c3">
								<p>33</p>
							</entry>
							<entry colname="c4">
								<p>203</p>
							</entry>
						</row>
						<row>
							<entry colname="c1">
								<p>NR-MSP-PEI ads.</p>
							</entry>
							<entry colname="c2">
								<p>298</p>
							</entry>
							<entry colname="c3">
								<p>15</p>
							</entry>
							<entry colname="c4">
								<p>266</p>
							</entry>
						</row>
						<row>
							<entry colname="c1">
								<p>NR-MSP-PEI graf.</p>
							</entry>
							<entry colname="c2">
								<p>388</p>
							</entry>
							<entry colname="c3">
								<p>23</p>
							</entry>
							<entry colname="c4">
								<p>227</p>
							</entry>
						</row>
						<row>
							<entry colname="c1">
								<p>NR-MSP-PEI-ACA</p>
							</entry>
							<entry colname="c2">
								<p>452</p>
							</entry>
							<entry colname="c3">
								<p>&#8722;12</p>
							</entry>
							<entry colname="c4">
								<p>170</p>
							</entry>
						</row>
						<row rowsep="1">
							<entry colname="c1">
								<p>NR-MSP-PEI-SUCC</p>
							</entry>
							<entry colname="c2">
								<p>389</p>
							</entry>
							<entry colname="c3">
								<p>&#8722;29</p>
							</entry>
							<entry colname="c4">
								<p>511</p>
							</entry>
						</row>
					</tbody>
				</tgroup>
			</table>
			<p>As a basis for comparison, these particular S-MSPs and NR-MSPs were chosen due to their similarity in size as determined from DLS methods on the nonfluorescent particles (see Figure S1 in Additional file 
				<supplr sid="S2">2</supplr>), i.e., around 500&#8201;to approximately&#8201;600&#8201;nm by DLS as well as electron microscopy images (Figure&#8201;
				<figr fid="F3">3</figr>). DLS for fluorescently labeled particles (Table 
				<tblr tid="T1">1</tblr>) is carried out to confirm redispersibility of the particles in aqueous solvent at a physiologically relevant pH (7.2) after all processing steps (synthesis, drying, solvent extraction/calcination and surface functionalization), as judged by the quality of the measurement as well as the polydispersity index. The DLS (<it>z</it>-average) values listed in Table 
				<tblr tid="T1">1</tblr> are thus based on an average of three good quality measurements, thus confirming full redispersibility of all particles in HEPES buffer solution at pH 7.2, which was chosen because it is also used to buffer cell media in the cellular experiments. The DLS values listed in Table 
				<tblr tid="T1">1</tblr> cannot, however, be used to determine the hydrodynamic size in solution in this case as the fluorescent labeling may distort the calculations applied to derive size from light scattering measurements. Moreover, DLS cannot be correctly applied to derive the hydrodynamic size for non-spherical particles. Thus, the particle sizes and morphologies were rather determined by scanning electron microscopy (Figure&#8201;
				<figr fid="F3">3</figr>). For the rod-like particles, the aspect ratio (AR) was determined to be 3 to 4 based on SEM analysis. Since no shape variety was observed for spherical particles, the aspect ratio is regarded as 1.</p>
			<suppl id="S2">
				<title>
					<p>Additional file 2</p>
				</title>
				<text>
					<p>
						<b>Figure S1</b> DLS measurements of nonfluorescent NR-MSPs (red) and S-MSPs (green) measured in water after SDA removal and drying.</p>
				</text>
				<file name="1556-276X-7-358-S2.tiff">
   <p>Click here for file</p>
</file>
			</suppl>
			<fig id="F3"><title><p>Figure 3 </p></title><caption><p>Electron microscopy images of the produced mesoporous silica particles</p></caption><text>
   <p><b>Electron microscopy images of the produced mesoporous silica particles. (a)</b> TEM image of sample S-MSP<sub>1</sub> illustrating the porous structure, <b>(b)</b> SEM image of samples S-MSP<sub>1</sub>, <b>(c)</b> S-MSP<sub>2</sub> and <b>(d)</b> NR-MSP.</p>
</text><graphic file="1556-276X-7-358-3"/></fig>
			<p>From the transmission electron microscopy image (Figure&#8201;
				<figr fid="F3">3</figr>a), the mesoporous structure of the particle can also be deduced. The porous structure was also confirmed by powder X-ray scattering and nitrogen sorption measurements (Figure&#8201;
				<figr fid="F4">4</figr>), from which the different pore size characteristics are also clearly observed. The S-MSPs were templated using cetyltrimethyl ammonium surfactants, typical of a MCM-41 synthesis, which in our reported case resulted in pore size of 3.5&#8201;nm (by Density functional theory (DFT)) and unit cell parameter of 4.7&#8201;nm (for S-MSP<sub>1</sub> and S-MSP<sub>2</sub>). On the other hand, the SDA used for the synthesis of NR-MSP, the nonionic surfactant block-co-polymer P123 typical for the synthesis of SBA-15 materials, results in pore sizes of 7&#8201;nm and over in case additives are used 
				<abbrgrp>
					<abbr bid="B23">23</abbr>
					<abbr bid="B25">25</abbr>
				</abbrgrp>. In this case, the pore size of the NR-MSP is 11.3&#8201;nm (by DFT) with a unit cell parameter of 14.8&#8201;nm. Mesoporous silica nanorods have also been synthesized using CTAB as structure-directing agent with another nonionic surfactant, peregal Os-25, as co-template 
				<abbrgrp>
					<abbr bid="B26">26</abbr>
				</abbrgrp>. On an interesting note, rod-shaped SiC has also been prepared using uncalcined mesoporous silica SBA-15 as template 
				<abbrgrp>
					<abbr bid="B27">27</abbr>
				</abbrgrp>. The advantage with our applied synthesis regime, besides the exceptionally large pores that can be obtained, is the very short synthesis time (1&#8201;h) 
				<abbrgrp>
					<abbr bid="B23">23</abbr>
				</abbrgrp>.</p>
			<fig id="F4"><title><p>Figure 4 </p></title><caption><p>Structural characteristics of the two different mesophases studied</p></caption><text>
   <p><b>Structural characteristics of the two different mesophases studied. (a)</b> Powder X-ray diffraction (PXRD) pattern of a typical S-MSP structure with hexagonally arranged pores (lattice spacing&#8201;=&#8201;4.7&#8201;nm), <b>(b)</b> PXRD pattern of NR-MSP exhibiting hexagonal order with lattice spacing of 14.8&#8201;nm, <b>(c)</b> N<sub>2</sub>-sorption isotherm for S-MSP and <b>(d)</b> N<sub>2</sub>-sorption isotherm for NR-MSP, both of characteristic IUPAC type IV for mesoporous materials.</p>
</text><graphic file="1556-276X-7-358-4"/></fig>
			<p>The fluorescent labeling of the particles regardless of method (co-condensation or post-synthesis grafting) were successful, as determined by fluorescence intensity measurements in HEPES buffer at the same concentrations (0.5&#8201;mg/ml; Table 
				<tblr tid="T1">1</tblr>). On a related note, we want to highlight the alteration of fluorescence intensity upon surface functionalization when fluorescein is used as the fluorescent tag. Fluorescein, mostly used in the &#8216;activated&#8217; form FITC, is a pH probe, and thus, both its absorption and fluorescence properties vary with pH as well as solvent 
				<abbrgrp>
					<abbr bid="B28">28</abbr>
				</abbrgrp>. This not only has implications for its intracellular localization upon quantification of cellular uptake as the pH in different cellular compartments differ, and for instance, in endo/lysosomes where particles would reside as a result of endocytotic uptake, the environment is acidic (pH 5 to 6). As is clearly illustrated in Table 
				<tblr tid="T1">1</tblr>, surface functionalization, especially with acidic/basic groups such as amines or carboxylic acids (PEI and SUCC) which are the mostly used derivatizations when further bioconjugation is aimed for, also results in local pH changes on the nanoparticle surface. This has direct implications for differences in fluorescence intensity of the nanoparticles, despite being based on the same particle and measured at the same pH (here, in HEPES buffer at pH 7.2). This complicates fluorescence intensity-based quantification of cellular uptake as intracellular localization of the particles is not known at the time of detection whereby fluorescence intensity could also be measured at the right pH, and moreover, the localization for all particles within the same cell is not necessarily coinciding. Nevertheless, despite this drawback, fluorescein is the most widely used fluorescent tag due to its low cost, and these limitations in the absolute quantification based solely on fluorescence intensity are rarely taken into account. Consequently, we have chosen to mainly focus on percentage of positive cells in our cellular uptake studies as this value is not dependent on the absolute intensity of the particles.</p>
			<p>Moreover, surface functionalization may also alter the intracellular localization of particles (Figure&#8201;
				<figr fid="F5">5</figr>) as, for instance, PEI is commonly used as a nonviral gene transfection agent due to its ability to destabilize endosomal membranes and promote endosomal escape 
				<abbrgrp>
					<abbr bid="B29">29</abbr>
				</abbrgrp>. When compared to the uncoated spherical S-MSP<sub>1</sub>, indeed a more diffuse &#8216;spread-out&#8217; pattern can be discerned for the PEI-coated particle, whereas a clearer intracellular aggregation of particles is seen when no PEI is present. This may be due to the fact that uncoated particles (Figure&#8201;
				<figr fid="F5">5</figr>b) are more compartmentalized inside the cells as compared to their PEI-functionalized counterparts, which are more efficiently capable of escaping endo/lysosomes and consequently able to distribute inside the whole cell (cytoplasm). For the rod-like NR-MSPs, however, an almost fibrous pattern can be perceived, indicative of individual internalized rods (Figure&#8201;
				<figr fid="F5">5</figr>).</p>
			<fig id="F5"><title><p>Figure 5 </p></title><caption><p>Cellular uptake of particles as studied by confocal fluorescence microscopy</p></caption><text>
   <p><b>Cellular uptake of particles as studied by confocal fluorescence microscopy.</b> Cellular uptake of uncoated rods <b>(a</b> and <b>b)</b> and spheres <b>(c</b> and <b>d)</b> vs PEI-functionalized S-MSPs <b>(e</b> and <b>f)</b> (spheres) in HeLa cells after 4&#8201;h incubation, resulting in different intracellular distribution patterns. All images are confocal sections thorough the nucleus.</p>
</text><graphic file="1556-276X-7-358-5"/></fig>
			<sec>
				<st>
					<p>Cellular uptake of uncoated particles</p>
				</st>
				<p>Cellular uptake was first studied on uncoated particles with different morphology in order to find out if shape effects could only result in different extents of internalization. The method of investigation was fluorescence-assisted cell sorting (FACS). The MFI values can be found in Additional files 
					<supplr sid="S3">3</supplr>
					<supplr sid="S4">4</supplr> and 
					<supplr sid="S5">5</supplr> for reference. We note that MFI could benefit from being normalized against particle-specific fluorescence before drawing any conclusions, and these values can also be found in Additional files 
					<supplr sid="S3">3</supplr> and 
					<supplr sid="S4">4</supplr>. To broaden our observations, percentage of positive cells were furthermore determined for two different cell lines to investigate whether distinctions can be made based on cell origin also. Thus, two cancer cell lines were chosen for this purpose: HeLa cervical cancer cells and Caco-2 human epithelial colorectal adenocarcinoma cells. The Caco-2 cell lines are heterogenous and easily polarized when cultured under specific conditions, whereas HeLa are homogenous cells with a fibroblastic morphology. Cellular morphology could also influence uptake behavior, which is why we chose to study these two particular cell lines. Additionally, three different concentrations, 10, 2 and 1&#8201;&#956;g/mL, were studied to find concentration-related differences. It is worth to mention that MSNs are frequently studied <it>in vitro</it> at concentrations up to 100&#8201;&#956;g/mL, so our chosen concentrations are fairly low. As our particle sizes are also larger than in typical MSN studies (100 to approximately 200&#8201;nm), this also means that the number of particles used in our experiments is much lower than those in most studies to date. In order to detect internalized particles only, the extracellular fluorescence was quenched with trypan blue 
					<abbrgrp>
						<abbr bid="B30">30</abbr>
					</abbrgrp> in both microscopy and FACS studies. The resulting uptake of uncoated particles of different morphology in the two different cell lines at two different concentrations is illustrated in Figure&#8201;
					<figr fid="F6">6</figr>.</p>
				<suppl id="S3">
					<title>
						<p>Additional file 3</p>
					</title>
					<text>
						<p>
							<b>Figure S2</b> MFI values from FACS for HeLa cells incubated with 10 and 2&#8201;&#956;g/mL MSPs for 4&#8201;h. The lower graphs have been normalized against pure particle suspension fluorescence values measured at 530&#8201;nm in HEPES buffer at pH 7.2.</p>
					</text>
					<file name="1556-276X-7-358-S3.tiff">
   <p>Click here for file</p>
</file>
				</suppl>
				<suppl id="S4">
					<title>
						<p>Additional file 4</p>
					</title>
					<text>
						<p>
							<b>Figure S3</b> MFI values from FACS for Caco-2 cells incubated with 10 and 2&#8201;&#956;g/mL MSPs for 4&#8201;h. The lower graphs have been normalized against pure particle suspension fluorescence values measured at 530&#8201;nm in HEPES buffer at pH 7.2.</p>
					</text>
					<file name="1556-276X-7-358-S4.tiff">
   <p>Click here for file</p>
</file>
				</suppl>
				<suppl id="S5">
					<title>
						<p>Additional file 5</p>
					</title>
					<text>
						<p>
							<b>Figure S4</b> MFI values from FACS for HeLa cells incubated with 1&#8201;&#956;g/mL MSPs for 4&#8201;h. The right graph has been normalized against pure particle suspension fluorescence values measured at 530&#8201;nm in HEPES buffer at pH 7.2.</p>
					</text>
					<file name="1556-276X-7-358-S5.tiff">
   <p>Click here for file</p>
</file>
				</suppl>
				<fig id="F6"><title><p>Figure 6</p></title><caption><p>Cellular uptake of uncoated MSPs in two different cancer cell lines after 4-h incubation</p></caption><text>
   <p><b>Cellular uptake of uncoated MSPs in two different cancer cell lines after 4-h incubation. (a)</b> HeLa 10&#8201;&#956;g/ml, <b>(b)</b> HeLa 2&#8201;&#956;g/ml, <b>(c)</b> Caco-2 10&#8201;&#956;g/ml and <b>(d)</b> Caco-2 2&#8201;&#956;g/ml; NR-MSP (green), S-MSP<sub>1</sub> (pink) and S-MSP-2 (blue). The shaded area is the control (no particles).</p>
</text><graphic file="1556-276X-7-358-6"/></fig>
				<p>Clearly, there is a preference by both cell lines for rod-shaped particles (green histograms) as compared to spherical particles (Figure&#8201;
					<figr fid="F6">6</figr>). This is less evident for HeLa cells at 10&#8201;&#956;g/ml if only positive cell percentage values are regarded (see Figure&#8201;
					<figr fid="F7">7</figr>) but more clearly so for the histogram plots (Figure&#8201;
					<figr fid="F6">6</figr>). The observed high uptake is also corroborated by the microscopy results illustrated in Figure&#8201;
					<figr fid="F5">5</figr>. Importantly, the differences in peak shift should also not exclusively be due to differences in fluorescence intensity between the particles as the inherent fluorescence for NR-MSP and S-MSP<sub>1</sub> are similar (approximately 600; Table 
					<tblr tid="T1">1</tblr>). It is interesting to note the bimodal peak distribution of S-MSP<sub>1</sub>, whereas the peak for S-MSP<sub>2</sub> in all cases is not largely shifted from the control, indicating very low uptake. This distinction between the two spherical S-MSPs probably lies in the surface charge as S-MSP<sub>1</sub> is negatively charged to resemble that of pristine silica materials, whereas S-MSP<sub>2</sub> is a co-condensed material consisting of basic aminopropyl groups giving rise to positive charge at neutral pH. These abundant amino groups counteract the acidic silanol groups responsible for the negative charge of silica surfaces, thus resulting in a net neutral charge under the studied conditions. As the NR-MSPs were post-synthesis-functionalized with FITC-APTES in just enough amount to yield a sufficient fluorescent labeling, the surface of this material also resembles that of pure silica (and S-MSP<sub>1</sub>). It is noteworthy that previous MSN reports studying rod-like particles in a biological setting have also been fluorescently labeled according to similar protocols, so our S-MSP<sub>1</sub> and NR-MSP results can advantageously be compared to those. Indeed, the same trend that rod-like particles is preferred over spherical ones is observable in our results, perfectly in line with earlier reports as discussed in the &#8216;Background&#8217; section. The difference in uptake between the spherical particles (S-MSP<sub>1</sub> and S-MSP<sub>2</sub>), observed in both cell lines, is also interesting. It has been proposed that serum protein adsorption onto particles, coronation, leads to enhanced unspecific cellular uptake and that high charge, whether negative or positive, results in increased protein adsorption. In light of this, the two negatively charged particles S-MSP<sub>1</sub> and NR-MSP could be subject to higher protein adsorption (from the cell media), which could lead to increased cellular uptake. On the other hand, a near-neutral charge such as the one observed for S-MSP<sub>2</sub> also indicates diminished electrostatic dispersion stabilization, which could lead to particle aggregates that are too large for the cells to take up. Furthermore, as the particles are uncoated, no steric stabilization is provided, and thus, this particular MSP system may be susceptible to aggregation in the physiological environment.</p>
				<fig id="F7"><title><p>Figure 7 </p></title><caption><p>Cellular uptake efficiency</p></caption><text>
   <p><b>Cellular uptake efficiency.</b> Cellular uptake of coated vs uncoated (nc) rods vs spheres in HeLa (<b>(a)</b> 10&#8201;&#956;g/ml and <b>(b)</b> 2&#8201;&#956;g/ml) vs Caco-2 (<b>(c)</b> 10&#8201;&#956;g/ml and <b>(d)</b> 2&#8201;&#956;g/ml) cell lines after 4&#8201;h incubation, as measured by FACS. Error bars represent SD (<it>n</it>&#8201;&#8805;&#8201;4). The pink dotted line distinguishes the rods from the spheres.</p>
</text><graphic file="1556-276X-7-358-7"/></fig>
			</sec>
			<sec>
				<st>
					<p>Cellular uptake of organically modified particles</p>
				</st>
				<p>Organic modification is almost exclusively required to obtain desirable properties for a MSN system in order to provide for eligible biobehavior. The added value in organic modification may include dispersion stability, surface charge tuning, stealth properties, anchoring points for biofunctionalization (antibodies, proteins, peptides, targeting ligands and drug molecules), increased hydrophilicity, molecular gate-keeping, stimuli responsiveness, controlled cleavage of surface-bound coating or moieties, and so forth. On a less sophisticated level, it is generally believed that a net positive charge is beneficial in maximizing cellular uptake due to attraction to the negatively charged cell membrane. Thus, functionalization with positively charged surface groups is frequently applied to enhance cellular uptake. This is also the primary reason why we decided to functionalize our particles with the cationic polyelectrolyte PEI. Aside from enhanced cellular uptake, the branched structure of PEI also offers a higher amount of terminal primary amino groups than possible to attain via conventional amino functionalization, simultaneously providing increased electrostatic suspension stability to the system and possibly introducing pH-dependent molecular gate properties along with enabling endosomal escape ability, both of which would be utilized when carrying drug cargo for intracellular release 
					<abbrgrp>
						<abbr bid="B31">31</abbr>
					</abbrgrp>. To investigate the effect on cellular uptake upon derivatization of the PEI layer, we also capped the terminal primary amino groups with either uncharged acetyl groups or acidic (negatively charged under neutral conditions) succinic acid groups. The uptake in terms of positive cell percentage of the whole series of particles with (or without) different functionalization is presented in Figure&#8201;
					<figr fid="F7">7</figr>.</p>
				<p>For HeLa cells, the uptake is efficient to a degree that no differences between surface-modified NR-MSPs could be detected even at concentrations as low as 2&#8201;&#956;g/ml, whereas a decreased uptake of (uncoated) spheres was observed also at 10&#8201;&#956;g/ml. For all other particles, the uptake was virtually 100% for both concentrations. For Caco-2 cells, the differences were clearer and followed what could be expected regarding surface-charge-induced differences. Capping the charge with uncharged groups reduces the uptake, but a negative charge seems to reduce it even more. This effect is even more evident from the graph of normalized fluorescence intensity vs type of particles in Figure S3 in Additional file 
					<supplr sid="S4">4</supplr>, where MFI values from FACS have been normalized against particle-specific fluorescence in suspension. This observed effect is probably due to the fact that the absolute charge is not neutral, but still, a competition between negatively charged silanols on the underlying silica surface and secondary and tertiary amine groups in the PEI layer results in a net (overall) neutral effective charge. As this net effective charge recorded at neutral pH was even slightly negative, the capping of the terminal primary amines seems to have been very effective as it has been able to shield the positive charge. As the terminal acetyl groups are not charged, this &#8216;charge capping&#8217; possibly serves to reduce the enhancement in uptake observed for positively charged particles. This kind of charge capping consequently has also been used to reduce the toxicity associated with high molecular weight PEI when used as a gene carrier 
					<abbrgrp>
						<abbr bid="B24">24</abbr>
					</abbrgrp>. To account for this well-known PEI toxicity, as well as the notation that surface modification could have a profound impact on the cytotoxicity of the particles, cellular viability was also determined for the whole particle series (Figure&#8201;
					<figr fid="F8">8</figr>).</p>
				<fig id="F8"><title><p>Figure 8 </p></title><caption><p>Cell viability</p></caption><text>
   <p><b>Cell viability.</b> Viability of HeLa cells incubated with rod-like and spherical mesoporous silica nanoparticles at 12&#8201;h, assessed by a WST-1 assay. Error bars represent SD (<it>n</it>&#8201;&#8805;&#8201;3). Statistical analysis was made by ANOVA followed by a Dunnett's multiple comparison post-test. All data sets were compared with a negative cytotoxicity control of cell media with a particle vehicle (DMSO). The level of significance was set at a probability of *<it>p</it>&#8201;&lt;&#8201;0.001. NC, negative control; PC, positive control (calyculin A).</p>
</text><graphic file="1556-276X-7-358-8"/></fig>
				<p>On the other hand, the succinylation provides for terminal negatively charged groups on the organic layer which, together with the secondary and tertiary amine groups in the PEI layer (or any residual primary amines), make up an organic layer consisting of both negative and positive charges. Not only has succinylation of branched PEI shown to lead to a ten-fold decrease in toxicity observed for pure PEI 
					<abbrgrp>
						<abbr bid="B24">24</abbr>
					</abbrgrp> but such zwitterionic functionalization has also been suggested to minimize serum protein adsorption 
					<abbrgrp>
						<abbr bid="B32">32</abbr>
					</abbrgrp>, which could otherwise lead to increased unspecific uptake. Thus, it may not be the negative charge as such that reduces the uptake but the zwitterionic nature of the organic layer 
					<abbrgrp>
						<abbr bid="B33">33</abbr>
					</abbrgrp>. This is also supported by the higher uptake observed for the negatively charged uncoated particles (Figures 
					<figr fid="F6">6</figr> and 
					<figr fid="F7">7</figr>c,d) as compared to the net neutral S-MSP<sub>2</sub> consisting of a surface with negatively charged silanols and positively charged aminopropyl groups, which hardly exhibits any uptake at all. In Figure&#8201;
					<figr fid="F7">7</figr>, no distinctions for the rod-like particles can be deduced as they are all taken up almost in 100% of the cells, but for HeLa cells at even lower concentrations (1&#8201;&#956;g/ml), the charge-induced differences also start to occur as shown in the histogram presented in Figure&#8201;
					<figr fid="F9">9</figr> with the same trend, i.e., the positively charged rod-like particles are taken up to a greater extent. One interesting notation from both Figure&#8201;
					<figr fid="F9">9</figr> and the MFI values in Additional files 
					<supplr sid="S3">3</supplr>
					<supplr sid="S4">4</supplr> and 
					<supplr sid="S5">5</supplr> (normalized or not) is that the surface-polymerized PEI seems to be much more efficient in inducing cellular uptake of the rod-shaped MSNs as compared to the more commonly applied electrostatic adsorption of commercially available PEI. Thus, not only purely charge-induced effects but also the functionalization regime seems to be useful in fine-tuning the cellular uptake at lower doses as a &#8216;secondary&#8217; uptake regulator, if desired.</p>
				<fig id="F9"><title><p>Figure 9 </p></title><caption><p>Charge-induced differences in uptake</p></caption><text>
   <p><b>Charge-induced differences in uptake.</b> Incubation of NR-MSPs in HeLa cells at a low concentration (1&#8201;&#956;g/ml), NR-MSP (green, 83.6%), NR-MSP-PEI-ACA (red, 62.4%), NR-MSP-PEI-SUCC (orange, 69.6%), NR-MSP-PEI adsorbed (light blue, 93.2%), NR-MSP-PEI grafted (teal, 97.9%) and control (violet).</p>
</text><graphic file="1556-276X-7-358-9"/></fig>
			</sec>
		</sec>
		<sec>
			<st>
				<p>Discussion</p>
			</st>
			<p>Our observed enhanced uptake of the rod-like MSPs is in line with previous reports on rod-like MSN biobehavior. These previous reports have mainly concentrated on non-functionalized MSNs aside from the fluorescent labeling (i.e., comparable to our S-MSP<sub>1</sub> and NR-MSP) to render the particles observable by confocal (fluorescence) microscopy and other applied fluorescence-based characterization techniques. Meng et al. 
				<abbrgrp>
					<abbr bid="B13">13</abbr>
				</abbrgrp> investigated the aspect ratio effect on cellular uptake rate and amount, and found that particles with an AR of 2.1 to 2.5 were taken up in greater quantities than shorter (1.5 to 1,7) and longer (4 to 4.5) rods as well as spheres (AR&#8201;=&#8201;1), which seem consistent with earlier reports on organic nanoparticles for which AR&#8201;~&#8201;3 was found to be the most efficient in terms of cellular internalization 
				<abbrgrp>
					<abbr bid="B4">4</abbr>
				</abbrgrp>. The aspect ratio of our studied NR-MSP is around 3 to 4. Meng et al. stated that their observations implied that a cellular mechanism capable of discerning and responding to rod length was operative, and compared this observation to that of Champion and Mirtagotri 
				<abbrgrp>
					<abbr bid="B34">34</abbr>
				</abbrgrp>, who studied the phagocytosis mechanism of non-spherical polymer particles in macrophages and concluded that it was the local geometry (angle of curvature) at the point of contact with the cell membrane that initiated phagocytosis, not the overall AR. It is worth to mention that the two mechanisms of uptake studied in the two separate studies were different, though Meng et al. studied macropinocytosis and the effect of particle shape on this particular cellular uptake route in two cancer cell lines (HeLa and A549) 
				<abbrgrp>
					<abbr bid="B13">13</abbr>
				</abbrgrp>. Huang et al. also studied the effect of MSNs of different ARs (1, 2 and 4) on uptake amounts and rates in a human melanoma (A357) cell line as well as AR impacts on cellular function including cell proliferation, apoptosis, cytoskeleton formation, adhesion and migration 
				<abbrgrp>
					<abbr bid="B12">12</abbr>
				</abbrgrp>. They found that increasing AR gave rise to increased uptake whereas long rod-shaped particles could cause reorganization of the cytoskeleton, and ascribed this observation to the more efficient endocytosis of rod MSNs than spheres 
				<abbrgrp>
					<abbr bid="B12">12</abbr>
				</abbrgrp>. Whereas Meng et al. found the behavior to be similar between the two cancer cell lines studied 
				<abbrgrp>
					<abbr bid="B13">13</abbr>
				</abbrgrp>, Trewyn et al. found slight differences between cell lines when comparing a cancer cell line (Chinese hamster ovarian) to a human fibroblast cell line 
				<abbrgrp>
					<abbr bid="B16">16</abbr>
				</abbrgrp>. In our current investigation between two cancer cell lines, the overall trends seem to be similar but with different dose-dependencies. Huang et al. 
				<abbrgrp>
					<abbr bid="B14">14</abbr>
				</abbrgrp> studied the effect of uncoated and PEGylated MSNs with two different ARs (1.5 and 5) on biodistribution, clearance and biocompatibility <it>in vivo</it>, whereby they found that the AR affected the clearance rate in that short rod MSNs (AR&#8201;~&#8201;1.5) had a more rapid clearance rate than the long rod MSNs (AR&#8201;~&#8201;5). No profound <it>in vivo</it> toxicity (based on hematology, serum biochemistry and histopathology) was found, in line with their previous report where MSN concentrations as high as 1,000&#8201;mg/kg were used 
				<abbrgrp>
					<abbr bid="B35">35</abbr>
				</abbrgrp>. Another useful means of predicting <it>in vivo</it> compatibility when aiming for circulating nanoparticles is determining their hemolytic activity, whereby Yu et al. have investigated pure and amino-functionalized porous and non-porous silica nanoparticles of ARs 2, 4 and 8 and their cytotoxicity effects on macrophages (RAW 264.6), lung carcinoma cells (A549) and hemolysis of human erythrocytes 
				<abbrgrp>
					<abbr bid="B15">15</abbr>
				</abbrgrp>. The pure silica particles showed a porosity- and shape-dependency on hemolytic activity, with the porous MSNs with higher AR exhibiting reduced hemolytic activity, whereas for the amino-functionalized particles, the zeta potential (effective surface charge) was decisive 
				<abbrgrp>
					<abbr bid="B15">15</abbr>
				</abbrgrp>. On this note, we want to stress that as we have particles of distinctively different pore sizes (3 to 4&#8201;nm vs 11 to 12&#8201;nm), this might give rise to differences in hemolytic activity as it has also been pointed out earlier that porosity is a decisive property due to lower exposure of silanol groups to the cell membrane of a porous surface 
				<abbrgrp>
					<abbr bid="B36">36</abbr>
				</abbrgrp>. However, as surface modification eliminates this source of interaction, the porosity effect might be of subordinate importance for surface-modified MSPs. In the study by Yu et al., surface charge and porosity also governed cellular toxicity, whereas AR did not have any reported effect 
				<abbrgrp>
					<abbr bid="B15">15</abbr>
				</abbrgrp>. Also in our current study, no differences in cytotoxicity were observed at doses relevant for our experiments and higher (2.5 times our maximum used dose). We also note that the two different pore sizes of our chosen MSPs are rationalized based on applicability for different types of therapeutic cargo, whereby the 3- to 4-nm pores are ideal for the loading of small-molecular drugs, whereas the large-pore materials would also be suitable for carrying of biomacromolecules such as proteins (antibodies, enzymes, polypeptides and so on) and genes 
				<abbrgrp>
					<abbr bid="B37">37</abbr>
					<abbr bid="B38">38</abbr>
				</abbrgrp>. Finally, based on the troublesome nature of the fluorescein label, a more quantitative/absolute approach to studying the shape effect on nanoparticle uptake with nanomedical prospects and the efficiency of different particles in cargo delivery could constitute a more correlative approach. To date, this has been successfully measured in the extent of causing cytotoxicity upon delivery of the chemotherapeutic agent camptothecin or paclitaxel 
				<abbrgrp>
					<abbr bid="B13">13</abbr>
				</abbrgrp> or the efficacy of GFP knockdown 
				<abbrgrp>
					<abbr bid="B39">39</abbr>
				</abbrgrp> upon siRNA delivery, and similar approaches will also be pursued in our ongoing and future studies.</p>
		</sec>
		<sec>
			<st>
				<p>Conclusions</p>
			</st>
			<p>Porous silica particles of spherical and rod-like morphologies were studied for cellular uptake efficiency in two different cancerous cell lines for potential applications as nanomedical drug delivery carriers. According to the obtained results, both rod-like and spherical particles were readily internalized by HeLa cells with slight shape and charge-induced differences, whereas in Caco-2 cells, rod-shaped particles were internalized more efficiently. The difference was most pronounced for uncoated particles in both cell lines, whereby higher charge (S-MSP<sub>1</sub>) also induced higher uptake. A net positive charge (PEI) enhanced uptake regardless of shape and cell line. At lower doses, surface charge could be used to fine-tune the uptake even in HeLa cells, whereby higher charge (+/&#8722;) results in higher uptake over net neutral charge and positive over negative. At higher concentrations, the surface charge effect is overridden in HeLa cells, and rods are taken up despite coating or not, whereas for spheres and Caco-2 cells, distinctions can still be made. Uptake studies performed <it>in vitro</it> in different cell lines show that along with particle shape and surface functionalization, cellular origin and features may also influence the uptake of particles in cells. As shape seems to influence uptake in a cell-dependent manner, shape engineering could potentially be used as a tool for enhancing nanoparticle-mediated delivery.</p>
		</sec>
		<sec>
			<st>
				<p>Competing interests</p>
			</st>
			<p>The authors declare no competing interests.</p>
		</sec>
		<sec>
			<st>
				<p>Authors' contributions</p>
			</st>
			<p>DSK carried out the synthesis, functionalization and characterization of mesoporous silica nanoparticles, analyzed and interpreted characterization data and some part of the <it>in vitro</it> test results and has been involved in drafting and designing of the manuscript. DD carried out the <it>in vitro</it> tests such as cell viability, confocal microscopy and some part of the FACS studies, analyzed and interpreted the obtained <it>in vitro</it> results and has been involved in drafting and designing of the manuscript. RS studied the cellular uptake of sphere and rod-like MSPs at different concentrations in HeLa cell lines adopting FACS. EMJ carried out the synthesis and characterization of mesoporous silica nanorods and has been involved in drafting the manuscript. NR carried out the preliminary uptake and cytotoxicity studies of differently functionalized nanorods. MO designed and characterized the mesoporous nanorods in addition to revising the manuscript critically and contributing with important intellectual content. JEE provided biological lab facilities along with CS and DMT. CS has been involved in revising the manuscript critically for important intellectual content. DMT has been involved in providing the cell cultures and reagents for toxicity testing and revising the manuscript critically for important intellectual content. JMR conceived, designed and coordinated the study and drafted/wrote the manuscript. All authors read and approved the final manuscript.</p>
		</sec>
	</bdy>
	<bm>
		<ack>
			<sec>
				<st>
					<p>Acknowledgments</p>
				</st>
				<p>The Academy of Finland projects (#140193 JMR; #140759 and #126161, DMT; #137101, JMR, DD and NR), Centre of Excellence for Functional Materials (DSK), Centre for International Mobility India-Finland Fellowship (DD), Sigrid Juselius Foundation (RS, DMT), Nanolith Sverige AB (EJ and MO), FP7 IRG (DMT), &#197;AU Center of Excellence (DMT) and Liv och H&#228;lsa Foundation (DMT) are acknowledged for the financial support. Helena Saarento, Perttu Terho and Jari Korhonen are acknowledged for their technical assistance.</p>
			</sec>
		</ack>
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