In order to observe ultrastructure of insect sensilla, scanning and transmission electron microscopy (SEM and TEM, respectively) sample preparation protocol were presented in the study. Tween 20 was added into the fixative to avoid sample deformation in SEM. Fluorescence microscopy was helpful for improving slicing accuracy in TEM.
This report described sample preparation methods that scanning and transmission electron microscope observations, demonstrated by preparing appendages of the woodboring beetle, Chlorophorus caragana Xie & Wang (2012), for both types of electron microscopy. The scanning electron microscopy (SEM) sample preparation protocol was based on sample chemical fixation, dehydration in a series of ethanol baths, drying, and sputter-coating. By adding Tween 20 (Polyoxyethylene sorbitan laurate) to the fixative and the wash solution, the insect body surface of woodboring beetle was washed more cleanly in SEM. This study's transmission electron microscopy (TEM) sample preparation involved a series of steps including fixation, ethanol dehydration, embedding in resin, positioning using fluorescence microscopy, sectioning, and staining. Fixative with Tween 20 enabled penetrate the insect body wall of woodboring beetle more easily than it would had been without Tween 20, and subsequently better fixed tissues and organs in the body, thus yielded clear transmission electron microscope observations of insect sensilla ultrastructures. The next step of this preparation was determining the positions of insect sensilla in the sample embedded in the resin block by using fluorescence microscopy to increase the precision of target sensilla positioning. This improved slicing accuracy.
Scanning electron microscopy is an important tool in many morphology studies, that SEM shows surface structures1,2. Transmission electron microscopy's appeal is that it can be used to study a wide range of biological structures at the nanometer scale, from the architecture of cells and the ultrastructure of organelles, to the structure of macromolecular complexes and proteins. TEM shows inner structures3,4,5.
Coleoptera is the largest group of insects, including about 182 families and 350,000 species. Most of the coleopteran insects, in particular woodboring beetle, feed on plants, many of which are important pests of forests and fruit trees, causing devastating damage to trees6. At present, prevention and control population of pests based on chemical ecology theory have received increasing attention7. Efficient, low-toxic, pollution-free pheromone control methods have become an effective way8. Studying the sensilla morphology and ultrastructure of insects is an important part of insect chemical ecology research. The scanning and transmission electron microscopy (SEM and TEM, respectively) are used to great effect to study their morphology and internal anatomy. However, during preparation of insect samples for electron microscopy (EM), the objectivity and authenticity of the observation site may be affected9. In general, SEM sample preparation of insects requires cleaning, tissue fixation, dehydration, metathesis, drying, and sputter-coating10. Due to the complex environment in which woodboring beetle live, the body surface often has various pollutants and their appendages often have many fine long sensilla or bristles. In particular, some woodborers are not available from laboratory raising, which collected directly in the field, and then put into fixing fluid to ensure freshness and subsequently washed in the laboratory. If the sample is first fixed and then washed, obviously it is much more difficult to remove debris because glutaraldehyde strongly fixes it to the sample. Tween 20 is a surfactant11,12,13,14, which plays an important role in the washing process, including reducing the surface tension of water and improving the wettability of water on the surface of the laundry. In this study, Tween 20 was added to the fixing solution and PBS cleaning solution to reduce the surface tension of the liquid, and prevent the dirt from depositing on the body surface of the woodboring beetle, which made the body surface cleaner in SEM.
Using TEM, sensilla on different organs of insects can be sliced to reveal the clear structures inside them, thus providing a basis for analyzing sensilla functions. When the subject insect, such as woodboring beetle, is large, and its body wall has a substantial degree of sclerotization, so the fixative may not fully saturate organ tissues inside the insect body. Tween 20 can enhance the dispersion and suspension capacity of the dirt. In this study, Tween 20 was added to the fixative to enhance fixative fluid penetration into the insect body wall of woodboring beetle, avoiding deformation and collapse of the epidermi11,12,13. In addition, using general slicing technology, it is difficult to accurately locate different types of sensilla, in particular for some small sensilla15. Based on traditional TEM sample preparation, this study combined fluorescence microscopy and SEM to determine the position of insect sensilla in the embedded block, thus improving slicing accuracy.
CAUTION: Consult the material safety data sheets of reagents before using them. Several of the chemicals used during sample preparation are toxic, mutagenic, carcinogenic, and/or reprotoxic. Use personal protective equipment (gloves, lab coat, full-length pants, and closed-toe shoes) and work under a fume hood while handling the sample.
1. SEM Sample Preparation and Imaging
2. TEM Sample Preparation and Imaging
Figure 1: A fluorescent microscope photographed a resin block enclosing the appendage of the Chlorophorus caragana. (A) Antenna resin block; (B) Resin block at the end of the ovipositor. The arrow indicated the edge of the resin block; dotted circle indicates the target sensilla. Please click here to view a larger version of this figure.
Figure 2: Procedures of the precise sensilla location method. (A) The 4th sub-segment of a maxillary palp of Chlorophorus caragana, the dotted circle showed the sensilla targeted by SEM. (B) The 4th sub-segment of a maxillary palp of C. caragana viewed by fluorescence microscopy. White arrow showed the roughly cut edge of the resin block and the dotted circle showed the accurate location. (C) The marked distance from the edge of the resin block to the maxillary palp target location (28 µm in this sample). Please click here to view a larger version of this figure.
Using cleaning and fixative solution with Tween 20, cleaner SEM image was observed than that without Tween 20 (Figure 3). Tween 20 fixing solution penetrated the glutaraldehyde fixing solution into the tissue. Microtubule structure was clearly seen. TEM image of the internal structure of the sample was blurred without Tween 20 (Figure 4).
Figure 3: The sensilla locating on antenna of Chlorophorus caragana under SEM. Comparison of SEM image with Tween 20 (A) and without Tween 20 (B), which showed that picture A is cleaner than picture B in general. Please click here to view a larger version of this figure.
Figure 4: Chlorophorus caragana viewed by transmission electron microscopy of sensilla twig basiconica on the labial palps. Comparison of TEM image with Tween 20 (A) and without Tween 20 (B). Microtubule structure of picture A is clear, while that of picture B is blurred. Please click here to view a larger version of this figure.
We used SEM to study the types and ultrastructures of sensilla on the palps of C. caragana, finding 4 types of sensilla including 10 sub-types: 1 Böhm's bristles (BB.), 3 sensilla chaetica (Ch.1-Ch.3), 1 digitiform sensilla (Dig.), and 5 sensilla twig basiconica (S.tb.1-S.tb.5) (Table 1). Sensilla identification and ultrastructure was based on their morphology and size18,19,20,21,22,23. Our sample preparation methods rendered clear images of the surfaces and internal ultrastructures of insect sensilla.
Number | Type | Length (μm)a | Diameter at base (μm)a | Wall | Tip | Socket | Cuticular pores | Distribution |
1 | BB. | 5.18 ± 1.25 | 1.70 ± 0.47 | Smooth | Sharp | Wide | No | maxillary palp, labial palp |
2 | Ch.1 | 38.59 ± 8.20 | 3.15 ± 0.84 | Grooved | Sharp | Wide | No | maxillary palp, labial palp |
3 | Ch.2 | 81.54 ± 18.07 | 3.75 ± 0.88 | Grooved | Sharp | Wide | No | maxillary palp, labial palp |
4 | Ch.3 | 282.06 ± 22.60 | 6.10 ± 0.70 | Grooved | Sharp | Wide | No | labial palp |
5 | Dig. | 24.77 ± 2.98 | 1.24 ± 0.32 | Smooth | Blunt | Wide | No | maxillary palp |
6 | S.tb.1 | 6.51 ± 1.01 | 2.31 ± 0.25 | Grooved | With protrusions | Raised and tight | Tip pore | maxillary palp, labial palp |
7 | S.tb.2 | 5.91 ± 0.90 | 2.24 ± 0.30 | Smooth | Blunt | Raised and tight | Tip pore | maxillary palp, labial palp |
8 | S.tb.3 | 6.84 ± 0.98 | 1.96 ± 0.35 | Smooth | With protrusions | Raised and tight | Tip pore | maxillary palp, labial palp |
9 | S.tb.4 | 2.21 ± 0.59 | 2.86 ± 0.46 | Grooved | With protrusions | Raised | Tip pore | maxillary palp, labial palp |
10 | S.tb.5 | 1.16 ± 0.29 | 1.05 ± 0.19 | Smooth | Blunt | Raised and wide | Tip pore | maxillary palp, labial palp |
Table 1: Types of sensilla on the palps of C. caragana.
To examine the ultrastructure inside the sensilla on C. caragana palps, we used TEM. One example of these studies was continuous cross-sectional views of the peg of the S.tb.1 on maxillary palps. The views showed that the dendritic sheath surrounded the outer dendritic segments and extended until the tip pore (Figure 5A-D). Seven unbranched outer dendritic segments existed inside the inner receptor lymph cavity, which was surrounded by an outer cavity (Figure 5D). The tubular body was separated by a dendritic sheath from other outer dendritic segments at each sensillar socket base (Figure 5E). In the ciliary region, we noted 8 dendrites of different diameters, indicating the presence of 8 bipolar neurons. Finally, the ciliary segment contained 9 peripheral microtubule doublets (Figure 5F).
Figure 5: TEM views of sensilla type 1 twig basiconica (S.tb.1) on a Chlorophorus caragana maxillary palp30. (A) S.tb.1 with dotted lines marking regions close to the cross-sections taken for Figs. B-E. (B) Cross-section of finger-shaped protrusions showing scattered cuticula. (C) Cross-section of the basal region of finger-shaped protrusions showing inner receptor lymph cavities without outer dendritic segments. (D) Cross-section of the middle region of the peg showing the dendritic sheath dividing the sensillum-lymph cavity into both inner and outer cavities with 7 outer dendritic segments in the inner cavity. (E) Basal region of the peg showing the tubular body surrounded by a dendritic sheath and separated from outer dendritic segments. A tormogen cell forms the outside of the dendritic sheath. (F) Cross-section of the ciliary region showing 8 dendrites of different diameters. Abbreviations: bb, basal body; cs, ciliary segment; CW, cuticular wall; DS, dendritic sheath; iRL, inner receptor lymph cavity; M, microtubule; Mi, microvilli; oD, outer dendritic segment; oRL, outer receptor lymph cavity; S.tb.1, type 1 sensilla twig basiconica; TB, tubular body; TH, thecogen cell; TO, tormogen cell; TR, trichogen cell. Please click here to view a larger version of this figure.
In this article, we presented a sample preparation scheme for scanning and transmission electron microscopy for woodboring beetle. Using insect appendage as a representative study subject, we demonstrated several improvements over traditional sample preparation methods.
The liquid oil detached from the solid surface is emulsified into small droplets, which can be well dispersed and suspended in the washing medium to reduce redepositing on the surface of the object. Washing performance of surfactant includes all the basic characteristics such as wettability, permeability, emulsifying property, dispersibility, solubilization11,12,13,14. Effects of different detergents on the electron microscopic samples preparation of Golden Nematode showed that Tween 20 had the best cleaning effect, followed by sodium bicarbonate, and distilled water24. In this study, we found that Tween 20 can be used to reduce the surface tension of the liquid, and prevent the dirt from depositing on the body surface of the insect, in particular for woodboring beetle collected directly in the field. Insect body surface was washed more cleanly in SEM. Fixative with Tween 20 penetrated the insect body wall more easily, and subsequently better fixed tissues and organs in the body in TEM. The advantage of surfactant in electron microscopy sample preparation has been extensively studied24,25,26,27,28,29,30,31.
Also, we adopted a modified air-drying method for SEM sample preparation, in which the dehydrated sample was placed in a petri dish containing a silica gel desiccant that gradually evaporates the dehydrating agent. The biggest advantage of this method is that it is simple, easily maintained, and it keeps the microenvironment air dry and no special equipment required. The natural drying method is a simple, practical and effective method for seed, nut and long-term preservation of insect specimens. Although the sample volume shrinks during the natural drying process, the basic morphology of the sample is retained32. In general, Coleoptera insects have relatively low water content, and their surface is surrounded by hard chitin walls. Air-dry is able to meet requirements. However, this drying method is not suitable for the drying of tissues with a large water content, such as louse, mites, and larvae, because the surface tension will deform the sample during the drying process.
In order to observe and calculate the type and number of sensilla distributed across the surface of the appendage, dorsal, ventral and lateral of the appendage must be considered. Some sensilla were few, small, and sometimes covered, scan and observe carefully from all angles to find those sensilla fully protruding the epidermis or arising from the depression. Since many sensilla were relatively long and hairlike, the tip effect can be significant. So, the electron microscope acceleration voltage must not be too high, 5-20kV was best and we used 20kV.
In the TEM sample embedding, the sample had better close to the edge of the flat embedding moulds groovein order to save time when roughing the resin block. The traditional TEM method forcontinuously cutting the resin is extensive, and it is usually blindly cut using an optical microscope17,33. To improve on this, we first explored an insect sensilla localization technique in resin-embedded blocks by using fluorescence microscopy to view and measure the target distance to the cut. Compared with the traditional TEM trimming method, this technology can save sample preparation time and more accurately locate the target sensor. In the absence of measurement software, a scaled ruler can be placed in the field of view to roughly measure the target distance. The combination of an ultramicrotome with a fluorescence microscope provides clear observations of the cutting process, yielding accurate cuts of target sensilla and other appropriate subjects.
The authors have nothing to disclose.
We appreciate the generous assistance of the Beijing Vocational College of Agriculture, the Institute for the Application of Atomic Energy (Chinese Academy of Agricultural Science), the Bioresearch Center of Beijing Forestry University and Professor Shan-gan Zhang of the Institute of Zoology, Chinese Academy of Sciences. This research was supported by National Key R&D Program of China (2017YFD0600103), the National Natural Science Foundation of China (Grant No. 31570643, 81774015), Forest Scientific Research in the Public Welfare of China (201504304), Inner Mongolia Agricultural University High-level Talent Research Startup Plan (203206038), and Inner Mongolia Autonomous Region Higher Education Research Project (NJZZ18047), Inner Mongolia Autonomous Region Linxue "Double First-class" Construction Project (170001).
Anatomical lens | Chongqing Auto Optical limited liability company |
1425277 | |
Carbon adhesive tape | SPI Supplies, Division of Structure Probes, Inc. | 7311 | |
Carbon tetrachloride | Sigma | 56-23-5 | |
Copper grids | GilderGrids | G300 | |
Disodium hydrogen phosphate | Sinopharm group chemical reagent co., LTD | 10039-32-4 | |
Ethanol | J.T. Baker | 64-17-5 | |
Flat embedding molds | Hyde Venture (Beijing) Biotechnology Co., Ltd. | 70900 | |
Fluorescence microscope | LEICA | DM2500 | |
Glutaraldehyde | Sigma-Aldrich | 111-30-8 | Anhydrous EM Grade |
Isophorone | Sigma | 78-59-1 | |
Lead citrate | Sigma | 512-26-5 | |
Methanol | Sigma | 67-56-1 | |
Monobasic sodium phosphate | Its group chemical reagent co., LTD | 7558-80-7 | |
Objective micrometer | Olympus | 0-001-034 | |
Osmium tetroxide | Sigma | 541-09-3 | |
Petri dish | Aldrich | 1998 | |
Razor blade | Gillette | ||
Resin | Spurr | ERL4221 | |
Scalpel | Lianhui | GB/T19001-2008 | |
SEM | Hitachi | S-3400 | |
Silica gel desiccant | Suzhou Longhui Desiccant Co., Ltd. | 112926-00-8 | |
Small brush | Martol | G1220 | |
Sodium hydroxide | Sigma | 1310-73-2 | |
Sputter ion instrument | Hitachi Koki Co. Ltd., Tokyo, Japan | E-1010 | |
Stereo microscope | Leica | EZ4 HD | |
TEM | Hitachi | H-7500 | |
Tween 20 | Tianjin Damao Chemical Reagent | 9005-64-5 | |
Ultramicrotome | Leica | UC6 | |
Ultrasonic cleaner | GT Sonic | GT-X1 | |
Uranyl acetate | Sigma | 6159-44-0 |