Stable isotope imaging of biological samples with high resolution secondary ion mass spectrometry and complementary techniques
Introduction
As early as 1935, Schoenheimer et al. [1], [2] started using stable isotopes to study intermediary metabolism. Since then, stable isotope labelling has been used extensively to explore biological processes, often combined with mass spectrometry [3], [4] and Nuclear Magnetic Resonance [5], [6]. One advantage of using stable isotope labelling is that isotopic labels have little or no effect on the biochemical properties of the target molecules, so one can presume that stable isotope-labelled molecules behave in the same way as non-labelled molecules. The ability to carry out quantitative analysis with stable isotope labelling is also useful for fields like proteomics [7], [8]. However, most quantitative measurements of stable isotope ratios use bulk samples that have been extracted from whole tissues, making it impossible to draw conclusions about subcellular compartments or contributions of different cell types. Imaging the precise location of stable isotopes within cells by NanoSIMS can provide direct evidence of the distribution of labelled molecules and allow us to track molecules quantitatively as they interact with specific cells and tissues.
The CAMECA NanoSIMS 50 is a high-resolution secondary ion mass spectrometry (SIMS) instrument which can detect chemical and isotopic distributions with a lateral resolution of 50 nm. The instrument uses a 16 keV primary Cs+ beam to bombard the sample surface and collects at least five selected negative secondary ions using a Mauttach–Herzog mass analyzer with electrostatic sector and asymmetric magnet configuration [9]. The design of the NanoSIMS simultaneously optimizes high spatial resolution, high mass resolution, and high sensitivity, which makes it a powerful tool for studying many types of samples. The sensitivity can allow excellent analysis of species at concentrations of parts per billion for some analytes, which makes it particularly useful in imaging trace elements in cosmochemistry [10], [11], geology [12], [13], and plant science [14], [15]. The excellent mass resolution, m/Δm > 4500 with 80% transmission [16], enables quantitative analysis of stable isotopes even when there are close isobaric interferences, such as 12C1H− with 13C−, 12C15N− with 12C14N1H−, and 12C13C1H2− with 13C14N− [17]. Combining these instrumental advantages with stable isotope labelling, NanoSIMS analysis has proven useful for studying biological samples in the last decade. For instance, Thompson et al. [18] identified a symbiosis model between a cyanobacterium and unicellular alga by imaging the exchange of fixed 13C and 15N. Kraft et al. [19] used a NanoSIMS to observe, for the first time, phase separation in lipid mixtures. Lechene et al. [20], [21] studied the fixed nitrogen exchange between host and bacterial cells and quantitatively measured mammalian cardiomyocyte renewal. In biological studies, the most common stable isotopes used to label molecules are 2H, 13C, 15N, and 18O; all are readily imaged by the NanoSIMS [22], [23], [24], [25].
Due to the complexity of most biological problems, correlative techniques have been developed to extract as much information as possible from the samples. For instance, instruments have been designed to allow correlative fluorescence microscopy and electron microscopy [26], [27]. Some groups studying biological samples have used NanoSIMS in combination with fluorescence microscopy [28], in situ hybridization techniques [29], [30], transmission electron microscopy (TEM) [20], [31], atomic force microscopy (AFM) [19], [32], synchrotron techniques [14], ICP-MS [31], and electron probe microanalysis [15]. All of these techniques have provided useful information to understand complex biological mechanisms, such as phylogenetic identification of individual cells from fluorescence in situ hybridization [33], extremely sensitive and rapid imaging of trace elements over large areas from synchrotron X-ray fluorescence techniques [34], and subcellular morphology from TEM [20]. The techniques of backscattered electron (BSE) imaging in a scanning electron microscope (SEM) and AFM have been extensively developed in recent years so that they now have new capabilities that can be applied to studies with biological samples. For instance, low-voltage BSE imaging has been applied to study both the morphology of biological materials and to reconstruct 3-D images by tomography [35], [36], [37]. The excellent spatial resolution of AFM makes it easy to visualize single molecules [38], [39] and interactions between molecules [40], [41].
This article reports three recent investigations combining analysis in the NanoSIMS with site-specific correlative AFM and BSE imaging. We discuss the critical sample preparation protocols and experimental methods developed for imaging at the molecular, cellular, and tissue scale.
Section snippets
Molecule imaging
Supported lipid bilayers (SLBs) are attractive experimental models for fluid-phase membranes [42], [43] and can be conveniently prepared by well-established techniques.
Selecting the Cs+ dose in stable isotope Imaging
The Cs+ source in the NanoSIMS sputters the sample surface to generate the ionized signals to form the elemental images, but at the same time implants caesium into the sample. To achieve reliable quantification of stable isotopes and to obtain sufficiently high signals for imaging, pre-imaging implantation is needed because the yield of secondary ions depends on the surface concentration of Cs [9]. Fig. 1 shows how the counts for 12C− and 12C14N− vary as a function of Cs+ dose on a 5 nm
Conclusions
This article reports three applications of high-resolution stable isotope imaging with NanoSIMS where complementary techniques have been important in interpreting the SIMS data. Experiments have been carefully designed to ensure the imaged volumes with the selected techniques are as similar as possible so that we can be sure that the data from the different techniques is from exactly the same structures and organelles. AFM and NanoSIMS imaging on flat substrates can show topographic and
Acknowledgements
We thank Dr. Katie Moore and Mr. Clive Downing for suggestions on the NanoSIMS experiments; Dr. Sverre Myhra for suggestions on AFM experiments; Dr. Jean-Nicolas Audinot and Mr. Patrick Grysan for help on the correlative AFM and NanoSIMS imaging; Dr. Errin Johnson for suggestions on EM sample preparation; and Dr. Angelica Tatar for assistance in carrying out animal experiments. H. J is supported by a scholarship from the China Scholarship Council. L.G.F and S.G.Y are supported by grants from
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