Abstract
Magnetic nanoparticle-based sensors for MRI have been accelerated to a timescale of seconds using densely-functionalized particles of small size. Parameters that increase response rates also result in large nuclear magnetic relaxation rate and light scattering changes, allowing signals to be detected almost immediately after changes in calcium concentration.
Nanoscale biosensors are frequently based on the spatial reorganization of nanoparticle conjugates, which can give rise to a variety of optical or magnetic effects. Magnetic sensors involve magnetic nanoparticles (MNPs), which strongly affect the transverse relaxation time (T2) of water proton spins detected by nuclear magnetic resonance (NMR) spectroscopy or imaging (MRI). MNP conjugates have been engineered to undergo reversible analyte-dependent aggregation,1,2 where the analyte either reversibly cross-links particles itself or modulates binding between moieties attached to the nanoparticle surfaces. This mechanism has yielded sensors capable of producing R2 (= 1/T2) changes of up to two or threefold.3 Such changes can be detected at nanoparticle concentrations below 100 µM Fe, making MNP-based sensors an attractive alternative to MRI sensors based on T1 relaxation or other mechanisms. To date, MNP probes that undergo analyte-dependent assembly have been applied for a variety of in vitro NMR assays4 and as components of implanted biosensors for in vivo imaging.5
A serious but previously unaddressed limitation of MNP clustering-based sensors is their slow analyte response rates.6 Utility of MNP probes is compromised because of the long incubation times required to resolve substantial changes in R2 and because analyte concentration changes that take place much faster than the sensor response times cannot be detected. R2 changes initiated by addition of target analytes to MNP aggregation sensors have generally been reported to equilibrate over tens of minutes; this includes MNPs designed to cluster in the presence of glucose,2 calcium ions,1 and proteins.7 By comparison, unimolecular sensors detect analytes with response times on the order of seconds or even milliseconds.6
How can MNP aggregation kinetics be accelerated? We used the Smoluchowski aggregation-fragmentation formalism to model the dependence of MNP clustering on the characteristics of binary mixtures of particles assumed to interact via complementary surface-conjugated binding domains.6 Optimal rates were predicted when the density of surface functionalization moieties was highest for each MNP. Rates were also predicted to increase for constant MNP volume fraction by using smaller particles. Although the minimum size of interacting nanoparticles is restricted by the physical requirements for effective imaging agents, binary aggregating systems can be constructed by pairing MNPs with smaller crosslinking species.2 Monte Carlo simulations (Fig. 1) predicted that asymmetric binary systems with similar total particle surface area exhibit roughly twofold faster clustering kinetics than binary systems with two equal particle sizes.
We implemented strategies predicted to enhance MNP sensing kinetics by adapting a prototypical MNP-based calcium ion sensor presented in an earlier study.1 In this sensor, two different nanoparticle species are prepared separately by conjugation to the calcium-binding protein calmodulin (CaM) and to a peptide (RS20) that binds CaM only in its Ca2+-complexed form. Calcium therefore promotes multivalent binding between complementary particles and reversible clustering with an effective Ca2+ dissociation constant of ~1 µM. CaM and RS20 were incorporated into a new MNP platform with reduced particle size, increased protein surface conjugation density, and an asymmetric binary clustering mechanism.
Small, stable, and highly functionalized MNPs were prepared using a novel coating approach (Fig. 2a), based on photocrosslinking of diacetylene-containing lipids.9 Oleate-stabilized iron oxide cores were mixed with 1,2-bis(10,12-tricosadiynoyl)-sn-glycero-3-phosphoethanolamine-N-[maleimide(polyethylene glycol)-2000] (23:2 diyne PE-PEG-maleimide), and transferred to aqueous solvent. The resulting lipid-coated particles were subjected to ultraviolet (UV) irradiation at 254 nm for 40 minutes. Progress of the reaction was indicated by UV-visible spectroscopy (Fig. 2b), and the resulting photocrosslinked lipid-coated iron oxide (pcLCIO) nanoparticles were purified by ultracentrifugation to remove micelles and empty liposomes. Particles were characterized by transmission electron microscopy, which indicated electron dense core diameters of 5–10 nm, and by DLS, which indicated a total particle diameter of 16 ± 3 nm (Fig. S1), considerably smaller than commonly used dextran-coated superparamagnetic particles. Enhanced stability of the pcLCIO particles vs. uncrosslinked particles was confirmed by comparing their resistance to liposome-disrupting conditions10 (Fig. 2b, inset), as well as functional tests of calcium sensing properties; these tests revealed that sensors formed from uncrosslinked lipid-coated particles11 were susceptible to apparent degradation by metal chelators and to spontaneous calcium-independent dissociation of clusters (Fig. S2).
The pcLCIOs were conjugated to CaM via a site-specifically incorporated N-terminal cysteine residue. Protein quantification showed that up to 0.13 µM CaM per 1 µM iron could be conjugated via thiol-maleimide chemistry. This suggests, together with the particle dimensions, that stoichiometries in the range of 102–103 CaM moieties per pcLCIO particle are attainable, corresponding to functionalization density on the order of one molecule/nm2, due to the fact that every lipid terminates in a potential conjugation site. MRI assessment of CaM conjugated pcLCIOs indicated a transverse relaxivity of 47 ± 4 (mM Fe)−1s−1, measured at 4.7 T.
Asymmetric binary calcium sensors were assembled by pairing CaM-pcLCIOs with a polyvalent engineered protein binding partner, rather than a second nanoparticle species (Fig. 2c). The binding partner was formed by fusing an enhanced version of the 28 kD fluorescent protein DsRed12 to the N-terminus of RS20 (Fig. 2c). DsRed forms obligate tetramers with a diameter of approximately 6 nm.13 DsRed-RS20 proteins displayed calcium-dependent clustering in combination with CaM-pcLCIOs, but the aggregation was difficult to reverse except at elevated ionic strength, suggesting that dissociation was hindered by calcium-independent electrostatic interactions. To address this problem, we introduced charge reversal mutations in the DsRed-RS20 construct (Fig. S3) and evaluated reversibility of the corresponding sensors formed by mixing with CaM-pcLCIOs. Sensor properties were progressively improved by mutations K249E, targeting a linker residue between the DsRed and RS20 moieties, and by K188E, at a superficial solvent-exposed residue on DsRed (Fig. 2d). A variant with both substitutions, DsRed-RS20.v3, was used for all further experiments.
Sensors formed from CaM-pcLCIOs and DsRed-RS20.v3 were characterized by DLS and MRI. Sensors initially in EDTA responded to addition of excess CaCl2 by forming clusters ~100 times larger than observed in EDTA (Fig. 2e). Increases in size coincided with decreases in T2-weighted MRI signal in the presence of the DsRed-RS20 species (Fig. 2e, inset).
Multiple cycles of clustering and declustering were observed by DLS upon successive additions of excess CaCl2 and EDTA (Fig. 3a). In each case, substantial size changes were apparent in seconds for aggregation at high [Ca2+] and within the ~3 s mixing dead time following EDTA addition for disaggregation at low [Ca2+] (Fig. 3a). The effective rate constant for clustering was 0.252 ± 0.004 min−1 for sensors containing 50 µM Fe, 12.5 µM DsRed-RS20.v3, and 3.75 µM CaM at 37 °C (Figure S4). We determined a midpoint for calcium responsiveness (EC50) ~1 µM Ca2+ for this sensor at steady state, which makes it applicable for the detection of biologically-relevant calcium fluctuations (Fig. S5). The dynamics of sensor clustering varied systematically as a function of CaM levels conjugated to CaM-pcLCIOs (0.006–0.13 µM CaM per µM Fe), with higher levels of CaM per particle resulting in faster and more pronounced aggregation (Fig. 3b), as predicted by the modeling studies.6 Conjugation density-dependent differences were particularly notable immediately following the mixing dead time, after which clustering was much more pronounced for the most highly functionalized CaM-pcLCIOs (> 10-fold DLS radius increase) than for the least functionalized.
Sensor response dynamics were also analyzed by MRI in microtiter plates. Figure 3d shows images obtained as a function of time during modulation of free Ca2+ concentrations. Calcium or EDTA was added five minutes before the first scan (the dead time for sample mixing and positioning in the scanner). An approximately threefold R2 change is observable in the initial acquisition. R2 values remain stable for several scans, and are then reversed again within ~5 minutes upon transition from low [Ca2+] to high [Ca2+] or vice versa. This is more than an order of magnitude faster than R2 equilibration times previously reported for MNP aggregation sensors. In particular, for prototypical Ca2+ sensors1 formed without regard for the kinetic optimization principles investigated here, R2 changes required roughly one hour to equilibrate, despite the use of twofold higher iron concentrations than employed for the experiments of Figure 3d (75 µM Fe).
These results show that robust analyte-dependent responses from nanoparticle aggregation-based probes can be detected within experimental dead times of seconds or minutes by DLS or MRI, respectively, indicating that these types of sensors are appropriate for measurements on biologically and chemically-relevant time scales faster than those previously explored. Examples of potential applications include the rapid in vivo detection of metabolites such as glucose, which can change by more than 10% within seconds in brain following stimulation14 or within minutes following food ingestion.15 In vitro diagnostic modalities based on magnetic4 or optically-detected16 nanoparticle aggregation could also be accelerated, allowing measurements to be made at intervals appropriate for rapidly developing clinical conditions such as anaphylaxis or stroke. Finally, although sensors with improved kinetics do not directly address the need for higher affinity detection of some biological targets, we note that accelerating the rate of responses to targets in general confers greater analyte sensitivity, according to mass action principles. The nanosensor design characteristics examined here, in addition to the novel photocrosslinked coating and electrostatic optimization we employed, could therefore find utility in a broad range of applications.
Supplementary Material
Acknowledgments
Funding Sources
ER was supported with the Beatriu Pinos Fellowship from the Government of Catalonia and SO was supported by an Uehara Memorial Foundation postdoctoral fellowship. Additional support was provided by NIH grants DP2-OD2114, R01-DA28299, R01-NS76462, and an MIT Simons Center seed grant to APJ.
Footnotes
Electronic Supplementary Information (ESI) available: [Supplemental Methods and References Sections and Figures S1, S2, S3, S4, and S5]. See DOI: 10.1039/c000000x/
Notes and references
- 1.Atanasijevic T, Shusteff M, Fam P, Jasanoff A. Proc. Natl. Acad. Sci. U S A. 2006;103:14707–14712. doi: 10.1073/pnas.0606749103. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 2.Sun EY, Weissleder R, Josephson L. Small. 2006;2:1144–1147. doi: 10.1002/smll.200600204. [DOI] [PubMed] [Google Scholar]
- 3.Josephson L, Perez JM, Weissleder R. Angew. Chem. Int. Ed. Engl. 2001;40:3204–3206. doi: 10.1002/1521-3773(20010903)40:17<3204::AID-ANIE3204>3.0.CO;2-H. [DOI] [PubMed] [Google Scholar]
- 4.Shao H, Min C, Issadore D, Liong M, Yoon TJ, Weissleder R, Lee H. Theranostics. 2012;2:55–65. doi: 10.7150/thno.3465. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 5.Ling Y, Pong T, Vassiliou CC, Huang PL, Cima MJ. Nat. Biotechnol. 2011;29:273–277. doi: 10.1038/nbt.1780. [DOI] [PubMed] [Google Scholar]
- 6.Shapiro MG, Atanasijevic T, Faas H, Westmeyer GG, Jasanoff A. Magn. Reson. Imaging. 2006;24:449–462. doi: 10.1016/j.mri.2005.12.033. [DOI] [PubMed] [Google Scholar]
- 7.Perez JM, Josephson L, O'Loughlin T, Hogemann D, Weissleder R. Nat. Biotechnol. 2002;20:816–820. doi: 10.1038/nbt720. [DOI] [PubMed] [Google Scholar]
- 8.Hütter M. J Colloid Interface Sci. 2000;231:337–350. doi: 10.1006/jcis.2000.7150. [DOI] [PubMed] [Google Scholar]
- 9.Johnston DS, Sanghera S, Pons M, Chapman D. Biochim. Biophys. Acta. 1980;602:57–69. doi: 10.1016/0005-2736(80)90289-8. [DOI] [PubMed] [Google Scholar]
- 10.Shamsai BM, Monbouquette HG. J. Memb. Sci. 1997;130:173–181. [Google Scholar]
- 11.Nitin N, LaConte LE, Zurkiya O, Hu X, Bao G. J. Biol. Inorg. Chem. 2004;9:706–712. doi: 10.1007/s00775-004-0560-1. [DOI] [PubMed] [Google Scholar]
- 12.Strack RL, Strongin DE, Bhattacharyya D, Tao W, Berman A, Broxmeyer HE, Keenan RJ, Glick BS. Nat. Methods. 2008;5:955–957. doi: 10.1038/nmeth.1264. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 13.Wall MA, Socolich M, Ranganathan R. Nat. Struct. Biol. 2000;7:1133–1138. doi: 10.1038/81992. [DOI] [PubMed] [Google Scholar]
- 14.Kiyatkin EA, Lenoir M. J. Neurophysiol. 2012;108:1669–1684. doi: 10.1152/jn.00521.2012. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 15.Dunn TC, Eastman RC, Tamada JA. Diabetes Care. 2004;27:2161–2165. doi: 10.2337/diacare.27.9.2161. [DOI] [PubMed] [Google Scholar]
- 16.Zhao W, Brook MA, Li Y. Chembiochem. 2008;9:2363–2371. doi: 10.1002/cbic.200800282. [DOI] [PubMed] [Google Scholar]
Associated Data
This section collects any data citations, data availability statements, or supplementary materials included in this article.